Search tips
Search criteria 


Logo of mmbrPermissionsJournals.ASM.orgJournalMMBR ArticleJournal InfoAuthorsReviewers
Microbiol Mol Biol Rev. 2002 March; 66(1): 122–154.
PMCID: PMC120783

Secretory Pathway of Trypanosomatid Parasites


The Trypanosomatidae comprise a large group of parasitic protozoa, some of which cause important diseases in humans. These include Trypanosoma brucei (the causative agent of African sleeping sickness and nagana in cattle), Trypanosoma cruzi (the causative agent of Chagas' disease in Central and South America), and Leishmania spp. (the causative agent of visceral and [muco]cutaneous leishmaniasis throughout the tropics and subtropics). The cell surfaces of these parasites are covered in complex protein- or carbohydrate-rich coats that are required for parasite survival and infectivity in their respective insect vectors and mammalian hosts. These molecules are assembled in the secretory pathway. Recent advances in the genetic manipulation of these parasites as well as progress with the parasite genome projects has greatly advanced our understanding of processes that underlie secretory transport in trypanosomatids. This article provides an overview of the organization of the trypanosomatid secretory pathway and connections that exist with endocytic organelles and multiple lytic and storage vacuoles. A number of the molecular components that are required for vesicular transport have been identified, as have some of the sorting signals that direct proteins to the cell surface or organelles in the endosome-vacuole system. Finally, the subcellular organization of the major glycosylation pathways in these parasites is reviewed. Studies on these highly divergent eukaryotes provide important insights into the molecular processes underlying secretory transport that arose very early in eukaryotic evolution. They also reveal unusual or novel aspects of secretory transport and protein glycosylation that may be exploited in developing new antiparasite drugs.


The Trypanosomatidae comprise a large group of parasitic protozoa, some of which cause important diseases in humans. These include Trypanosoma brucei (the causative agent of African sleeping sickness and nagana in cattle), Trypanosoma cruzi (agent of Chagas' disease in Central and South America), and Leishmania spp. (agent of visceral and [muco]cutaneous leishmaniasis throughout the tropics and subtropics). All of these parasites are transmitted by insect vectors and invade a range of different tissues or cell types in their mammalian hosts. Parasite survival within these environments requires the regulated surface transport of highly abundant coat glycoproteins and glycolipids as well as a large number of other, less abundant plasma membrane transporters, surface enzymes, and receptors that are delivered to the cell surface via a specialized invagination in the plasma membrane, termed the flagellar pocket. In this article we describe the ultrastructural organization of the trypanosomatid secretory pathway and review recent information on protein sorting signals that direct transport to the cell surface and the endocytic and lysosomal compartments, as well as the organization and function of glycosylation enzymes in the secretory pathway. As these parasites represent a highly divergent eukaryote lineage, these studies provide new insights into the extent to which the basic molecular machinery underlying secretory and endocytic processes has been conserved throughout eukaryotic evolution. Unusual features of the trypanosomatid secretory pathway, such as the polarized delivery of secretory material to the flagellar pocket and requirement for protein sorting to distinct lytic and storage vacuoles, as well as the presence of several unusual or unique glycosylation pathways are emphasized. A detailed understanding of these processes, some of which may represent adaptations of these organisms to parasitic lifestyles, may lead to the development of new antiparasitic strategies. The reader is also referred to other excellent reviews that have focused on particular aspects of protein trafficking in trypanosomatids (19, 61, 175, 250) and other protists (29).


Trypanosomatid parasites go through a number of distinct developmental stages during their digenetic life cycles in the insect vector and mammalian hosts (Fig. (Fig.1).1). The characteristic shapes of these developmental stages are maintained by an array of subpellicular microtubules that underlie the plasma membrane. A single flagellum emerges from a deep invagination in the plasma membrane, termed the flagellar pocket, that can be located either anterior (pro- and epimastigote stages) or posterior (trypomastigote stages) to the nucleus (Fig. (Fig.1).1). In some developmental stages (amastigote stages), the flagellum does not emerge from the flagellar pocket, while in others it may be tightly attached to the plasma membrane along the anterior-posterior axis of the cell. The flagellar pocket is a semisecluded compartment that is accessible to a range of proteins, including very large macromolecular complexes, but not to cellular components of the mammalian host immune system (250). The flagellar pocket membrane is not subtended by the subpellicular microtubule array and is thought to be the major site of exocytosis of secretory cargo (glycoproteins, proteoglycans, and glycolipids) that forms protective surface coats (Fig. (Fig.2).2). These surface coats are compositionally diverse but have a common feature in that they are all dominated by glycosylphosphatidylinositol (GPI)-anchored glycoproteins and/or free GPI glycolipids. The compositions of the surface coats of T. brucei, T. cruzi, and Leishmania spp. are briefly described below.

FIG. 1.
Life cycles of trypanosomatid parasites. The insect vectors for T. brucei, T. cruzi, and Leishmania are the tsetse fly (Glossina), the reduviid bug (Triatoma), and sand flies (Phlebotomus and Lutzomyia), respectively. The mammalian stages of T. brucei ...
FIG. 2.
Surface coats of trypanosomatids. The surface coats of trypanosomatid parasites are dominated by GPI proteins and/or non-protein-linked GPI glycolipids. The nature of the common and species-specific modifications (N-linked glycans, O-linked glycans, and ...

T. brucei

Early electron microscopy studies revealed that the plasma membrane of infective T. brucei bloodstream forms (BF) was covered in an electron-dense coat (357). This coat was subsequently shown to comprise a single ~58-kDa glycoprotein (approximately 107 copies/cell) termed the variant surface glycoprotein (VSG) (Fig. (Fig.2).2). The VSG coat protects the parasites from the alternative pathway of complement-mediated lysis, shields other cell surface proteins from the host immune system, and, by the process of antigenic variation, allows these parasites to persist for long periods in the host bloodstream (259). However, small proteins (e.g., trypsin) and essential nutrients can still permeate the VSG coat and reach the plasma membrane (42). Each VSG is attached to the plasma membrane by a GPI anchor that facilitates the dense packing of VSG dimers into coat arrays with minimal perturbation of the plasma membrane. The utilization of a GPI anchor may also allow VSGs to occupy spaces, such as the lipid core of polytopic transporters, from which integral membrane proteins may be excluded. The GPI anchors and N-linked glycans of VSG are variably modified with glycan side chains that further contribute to the function of the VSG as a macromolecular diffusion barrier (100, 210, 380). While VSG is evenly distributed over the plasma membrane (cell body, flagellum, and flagellar pocket), other GPI proteins on the surface of T. brucei BF can have a punctate distribution or be entirely restricted to the flagellar pocket (183, 238). The surface coat of T. brucei BF also contains a number of type 1 integral membrane proteins (the so-called invariant surface glycoproteins) (378) that likewise may be distributed over the entire cell body or sequestered within the flagellar pocket (Table (Table1).1). Finally, the plasma membrane contains a large number of polytopic transporters that underlie this surface coat and are inaccessible to surface antibodies in live trypanosomes (Table (Table1)1) (38).

Secretory pathway modifications of surface and secreted trypanosomatid antigens (only major proteins and glycoconjugates or proteins that have defined post-translational modifications are listed)

In contrast to T. brucei BF, the major insect (procyclic) stages of T. brucei are covered by a structurally distinct family of GPI proteins, termed the procyclins (287). The procyclins are encoded by multigene families and contain an extended rod-like polypeptide domain made up of repetitive amino acid sequences (EP procyclin contains 21 to 27 Glu-Pro repeats, while GPEET contains 5 or 6 Gly-Pro-Glu-Glu-Thr repeats) that terminate in a globular N-glycosylated N-terminal domain (287). The polypeptide backbone of the procyclins may be modified with phosphate groups (53, 209), while the GPI anchor is elaborated with large, branched poly-N-acetyllactosamine (poly-NAL) glycans (102). The poly-NAL chains on the GPI anchors are further capped with sialic acid by a cell surface trans-sialidase, conferring additional negative charges to the procyclin coat (53, 95, 209, 269). The procyclin coat is thought to protect this stage from hydrolases in the tsetse fly midgut and to be required for maturation to the metacyclic stage (354). It is therefore surprising that T. brucei procyclics lacking this surface coat, after deletion of a gene involved in GPI biosynthesis, survive in culture and can establish an infection (albeit slowly) in the tsetse fly (230). This is in contrast to the situation in BF, where deletion of GPI biosynthesis is lethal (230). However, it remains possible that the procyclins are still required for T. brucei infection of tsetse flies in the wild (where levels of infection are very low) and/or subsequent transmission to the mammalian host (99). The procyclic surface coat also contains a number of type 1 membrane proteins and flagellar pocket receptors (although fewer than in the BF stages), and it is likely that the procyclics contain a similar repertoire of plasma membrane transporters (Table (Table11).

T. cruzi

The surface coats of the major developmental stages of T. cruzi are dominated by two heterogeneous families of GPI-anchored glycoproteins, the mucin-like glycoproteins and the trans-sialidase family of glycoproteins (49, 67, 303) (Fig. (Fig.2;2; Table Table1).1). Both classes of glycoproteins are encoded by large multigene families. The mucins contain polypeptide backbones with Thr-rich domains that are extensively modified with short O-linked glycans (4, 9, 67, 109, 304) (Fig. (Fig.2).2). A primary function of some members of the trans-sialidase glycoproteins (60 to 250 kDa) is to transfer sialic acid from host glycoproteins to terminal galactose residues in the mucin O-linked glycans. Other members of this family lack trans-sialidase activity but may be important ligands for host cell receptors (49, 67). The sialylation of the mucin coat is thought protect the extracellular stages of T. cruzi from complement lysis and opsonization with anticarbohydrate antibodies in human serum and to play a role in T. cruzi invasion of a wide range of animal cells (49, 67, 261, 304). T. cruzi trypomastigotes invade animal cells by stimulating the fusion of secretory lysosomes with the plasma membrane of the target cell. After being internalized into these lysosomes, the trypomastigotes escape into the cytosol by secreting an acid-activated hemolysin (324). The surface trans-sialidases of the parasite facilitate this process by removing sialic acid from lysosomal membrane glycoproteins, thereby increasing the sensitivity of these membranes to the hemolysin. As the sialic acids are transferred to the trypomastigote coat, this process may also protect the parasite from its own hemolysin (133). In addition to the mucins and the trans-sialidase glycoproteins, T. cruzi trypomastigotes express a number of other GPI proteins that are involved in inactivating opsonic complement components (Table (Table1).1). Finally, all developmental stages of T. cruzi synthesize a highly abundant class of free GPIs (also referred to as glycoinositol-phospholipids [GIPLs] or lipopeptidophosphoglycan [LPPG]) that are likely to form a densely packed glycocalyx beneath the mucin coat (70, 71) (Fig. (Fig.22).

Leishmania spp.

The major surface macromolecule on the surface of the promastigote (insect) stage of Leishmania spp. is the hyperglycosylated GPI glycolipid, termed lipophosphoglycan (LPG) (205, 212). These molecules contain a highly conserved GPI anchor and a long phosphoglycan backbone that can be elaborated with species- and stage-specific glycan side chains (202, 205, 212). In all Leishmania spp. that are pathogenic in humans, LPG is expressed at very high levels (~5 × 106 molecules/cell) and forms a distinct glycocalyx that can be readily detected by electron microscopy (265). The LPG coat may protect the promastigote stage from lysis by the alternative complement cascade and extracellular hydrolases (277, 296) and may be a ligand, either directly or indirectly, for insect midgut and mammalian macrophage receptors (212, 297). Polymorphisms in LPG structure appear to contribute to the vector tropism of different Leishmania species (297). LPG is essential for the infectivity of Leishmania major promastigotes in both the insect and mammalian hosts (297, 335) but is dispensable for infectivity of Leishmania mexicana promastigotes in mice (152, 335, 351). The latter result may reflect functional redundancy with other surface molecules or differences in the stringency of the mouse model system for these different Leishmania species (152, 335, 351). The surface coat of Leishmania promastigotes also contains a number of GPI proteins and proteophosphoglycans (PPGs) (Table (Table1).1). Most of these proteins appear to be masked on live promastigotes by the LPG coat (166), and their precise function remains unclear. Leishmania donovani mutants lacking six of the seven gene copies for the major GPI protein, gp63 (promastigote surface protease, or leishmanolysin), are more sensitive to complement lysis (165). However, L. mexicana mutants lacking all GPI proteins can still establish an infection in animals (146, 165). Like T. cruzi, Leishmania promastigotes also synthesize very high levels of free GPIs that are 10-fold more abundant (~5 × 107 copies/cell) than LPG. While most of these glycolipids are found in the exoplasmic leaflet of the plasma membrane (201, 377), a significant pool may be located in the inner leaflet of the plasma membrane (280). These glycolipids are thus likely to be essential components of the surface coat, but their precise function remains unclear (Fig. (Fig.2).2). Attempts at obtaining GPI-negative Leishmania promastigotes were initially unsuccessful, suggesting that these glycolipids may be essential for viability (160). However, an L. mexicana mutant that is unable to synthesize all GPI-anchored macromolecules (protein and LPG) or mature free GPIs and that is viable in rich media has recently been generated (114). Remarkably, this mutant is weakly infective in animals, although this result is less surprising given that the mammalian (amastigote) stage of these parasites down-regulates the expression of most of these molecules and can acquire glycolipids from the host cell (200) (see below).

Leishmania spp. amastigotes reside within the phagolysosome compartment of mammalian macrophages and are unique amongst the trypanosomatids in lacking a prominent surface glycocalyx of GPI proteins or other GPI-anchored macromolecules (16, 200, 218, 265, 295, 370). Indeed, very few proteins can be labeled on the surfaces of live amastigotes by biotinylation and iodination protocols (370). Instead, this stage is coated with a surface layer of free GPIs and host-derived glycosphingolipids, most likely acquired from the inner leaflet of the macrophage phagolysosome membrane (200, 308, 343, 370). These glycolipids may protect essential plasma membrane transporters from proteolysis in the host cell lysosome, while the lack of surface-exposed proteins could constitute a form of immune evasion. Specifically, this surface architecture may reduce the opportunity for parasite peptides to be transported to the surface of infected macrophages in association with major histocompatibility complex class II proteins for presentation to the host T cells (249, 371).

Leishmania promastigotes and amastigotes also differ from other trypanosomatids in secreting copious amounts of soluble PPGs (153). The secreted (and surface-bound) PPGs characteristically contain very long polypeptide backbones which are modified with phosphoglycans similar to those added to LPG (157). Individually or after self-association, the PPGs form very large macromolecular filamentous structures that may facilitate promastigote aggregation and the transmission of large parasite clusters within the sand fly bite (340). The secreted PPGs may also deplete the level of lytic complement components in the mammalian lesion via nonproductive activation of the complement pathway (262) and modulate processes in the macrophage, such as the number and size of parasitophorous vacuoles and cytokine production (153, 263).


Early Secretory Pathway

Most proteins destined for the cell surface or lysosomes of trypanosomatids are initially assembled in the endoplasmic reticulum (ER). The ER is also the site of synthesis of most of the membrane phospho- and glycolipids. A number of markers for the trypanosomatid ER have been identified, including the major protein chaperones BiP and calreticulin, which assist newly synthesized proteins to fold in the ER lumen (21, 25, 164, 172), enzymes involved in the assembly of dolichol-linked oligosaccharides and GPI protein anchor precursors (54, 226, 271), and an ER-type Ca2+-ATPase that maintains high Ca2+ levels in the ER lumen (111, 189). In rapidly dividing trypanosomatids, the ER can account for 60% of the internal membranes (65). At the ultrastructural level the ER comprises the nuclear envelope and a connected system of cisternal or tubular membranes that are often closely associated with the plasma membrane (25, 159, 232, 265, 333, 365). These studies, as well as subcellular fractionation approaches, have revealed the presence of a number of functionally distinct ER subdomains. The first of these domains is the nuclear envelope that surrounds the large centrally located nucleus and remains intact throughout the cell cycle. Highly purified nuclei and nuclear envelopes have been isolated from T. brucei BF and procyclics and shown to contain numerous nuclear pore complexes that span the inner and outer membranes and are morphologically indistinguishable from those in the nuclear envelopes of other eukaryotes (290). One of the functions of the inner membrane is to maintain the organization of the nuclear lamina which contains the NUP-1 antigen, a large (350-kDa) coiled-coil protein that may be the trypanosomatid homologue of mammalian lamins (290). The outer membrane of the T. brucei nuclear envelope is studded with numerous ribosomes, suggesting that it is part of the rough ER (290). However, in Leishmania promastigotes, the nuclear envelope also contains a number of markers that are associated with a smooth ER fraction, suggesting that the nuclear envelope may comprise more than one domain (226). The cortical ER is continuous with the nuclear envelope but may also comprise a number of domains. These include the classical rough and smooth domains, which are often difficult to distinguish in electron micrographs because of the high density of free polysomes in the cytosol. However, two distinct ER domains can be resolved when L. mexicana promastigote microsomes are fractionated on sucrose density gradients. Both populations of microsomes contain the ER chaperone BiP (which is thought to be a marker of the entire ER), while the light fraction is highly enriched in enzymes involved in GPI and phospholipid biosynthesis (226). Light and electron microscopy studies indicated that these light and dense ER microsomal fractions form a mosaic throughout the cortical ER and nuclear envelope (226). Interestingly, some of these ER markers are transported to an unusual tubular compartment, termed the multivesicular tubule (MVT) in late-log- and stationary-phase promastigotes (226). Although initially thought to be part of the early secretory pathway, recent studies have shown that the MVT is a mature lysosome (120, 226, 365) (Fig. (Fig.3).3). In T. brucei and T. cruzi trypomastigotes, a distinctive subdomain of the smooth ER is consistently found attached to four specialized microtubules in the subpellicular array (357). These microtubules can be distinguished from other subpellicular microtubules based on their polarity and tubulin composition and directly underlie the flagellar attachment zone (FAZ) (127). Intimate connections between ER subdomains and the subpellicular microtubules also occur in other trypanosomatids that lack an adherent flagellum and FAZ (264). To date, no markers have been localized to these ER subdomains and their function is unknown.

FIG. 3.
Schematic representations of the secretory and endocytic organelles of T. brucei BF, T. cruzi epimastigotes, and Leishmania promastigotes. Most of the organelles involved in secretion and the early endocytic pathway are organized around the flagellar ...

Rapidly dividing trypanosomatids also contain a specialized transitional ER (tER) that lies directly opposite the single Golgi apparatus proximal to the flagellar pocket (Fig. (Fig.3).3). The tER comprises a cisternal extension of the cortical ER and is likely to be the major site at which proteins and lipids are exported to the Golgi (85, 103, 108, 226, 264, 365). A recent study on high-pressure-frozen L. mexicana promastigotes has provided remarkable new insights into the organization of the tER and its connection with the Golgi apparatus (365). The ribosome-free membrane of the tER facing the cis-Golgi contains many omega-shaped budding profiles, while the narrow space (100 nm) between the tER and the cis-Golgi is full of transport vesicles and an electron-dense matrix. There is no evidence that cytoskeletal elements are required for vesicular transport, although a single (or pair of) cytoplasmic microtubule(s) may be involved in maintaining the association of the tER with the Golgi (226, 365). This intimate association between the tER and Golgi may be essential to sustain the very high levels of protein and lipid transport to the cell surface. It is not known whether transport vesicles can also bud from other regions of the ER. However, in the absence of a conspicuous transcellular microtubule- or actin-based cytoskeleton in these parasites, these vesicles would have to reach the Golgi apparatus by the much less efficient process of diffusion (36).

Like its counterparts in other eukaryotes, the single Golgi apparatus of trypanosomatids consists of a stack of 3 to 10 cisternae and a polymorphic trans-Golgi network (TGN) (93, 108, 226, 365). Transport through the Golgi apparatus is thought to occur via two possible and not mutually exclusive mechanisms: vesicular transport between cisternae or the maturation and progressive movement of cisternae towards the trans face of the Golgi (cisternal maturation) (121). Cisternal maturation may be important in trypanosomatids, based on ultrastructural studies that show the apparent formation of new cisternae in the space between the tER and the cis face of the Golgi (365). Moreover, cisternal maturation may be required for the transport of very large macromolecular complexes, such as the filamentous PPGs of Leishmania promastigotes and amastigotes (341). The transport vesicles that are associated with the margins of the trypanosomatid Golgi may be involved in either the retrograde transport of resident proteins from older to younger cisternae or the anterograde transport of cargo proteins and lipids. Interestingly, and in contrast to the situation in animal cells, the Golgi apparatus of trypanosomatids and several other protists (32) does not break down during the cell cycle but undergoes medial fission during mitosis, along with other organelles (i.e., basal body, flagellum, kinetoplast, and mitochondria) (105, 365).

Only a few resident protein markers have been identified for the trypanosomatid Golgi (131, 184, 220). The fluorescent lipid BODIPY-ceramide has been used to label the Golgi in live T. brucei BF [105, 602], while this dye is specifically sequestered within the tubular lysosome of Leishmania promastigotes (159), highlighting possible differences in the lipid composition of secretory pathway membranes in different trypanosomatids. The different cisternae of the trypanosomatid Golgi appear to be biochemically and functionally differentiated, based on the polarized distribution of some Golgi marker proteins (56), the separation of different Golgi fractions in subcellular fractionation studies (125, 224), and differences in the cytochemical staining of some cisternae (94). Moreover, T. brucei BF glycoproteins receive complex N-linked glycan modifications that are assembled in different Golgi cisternae in animal cells (210, 252). Although the latter processing steps do not occur to the same extent in T. cruzi or Leishmania spp. (see below), many of the proteins in the latter species are modified with complex O-linked glycans or phosphoglycans by enzymes that also appear to be compartmentalized in the Golgi (131, 224). Some of these Golgi-specific processing steps can be inhibited with the ionophore monensin (20, 28), although this drug does not affect the surface transport of GPI proteins such as VSG (20, 85). Interestingly, brefeldin A, a fungal metabolite that induces the collapse of the Golgi into the ER in many animal cells and some other protozoa, has little or no effect on the structure of the Golgi or secretory transport in trypanosomatids (108) (K. A. Mullin and M. J. McConville, unpublished data). In T. cruzi epimastigotes, brefeldin A treatment actually results in an increase in the number of Golgi cisternae, a phenotype that is markedly more pronounced in T. cruzi mutants that are resistant to cysteine protease inhibitors (93). In this case, brefeldin A may affect post-Golgi sorting steps, including the recycling of lysosomal cargo receptors, leading to the accumulation of proteins in the early secretory pathway and the amplification of Golgi compartments.

The ER localization of several trypanosomatid proteins is likely to depend on the efficient retrieval of these proteins from the Golgi. For example, the T. brucei ER chaperone BiP contains a C-terminal tetrapeptide (MDDL [single amino acid code]) that is both necessary and sufficient for ER retention (21, 25). This motif also acts as an ER localization signal when appended to a secreted form of the green fluorescent protein (GFP) in L. mexicana promastigotes (159) (Fig. (Fig.4).4). By analogy with the HDEL/KDEL ER localization signal in Saccharomyces cerevisiae and animal cells, these proteins are probably recognized by a transmembrane receptor in the Golgi apparatus and recycled back to the ER in COP1 retrograde transport vesicles (316, 346). Similarly, some trypanosomatid ER membrane proteins (e.g., the ER-type Ca2+-ATPase [111]) contain a C-terminal KKXX motif that may direct these proteins into Golgi retrograde transport vesicles for delivery back to the ER. These observations support the notion that trypanosomatids have an efficient ER-to-Golgi retrograde transport pathway.

FIG. 4.
Secretory and endocytic organelles of L. mexicana promastigotes. Individual organelles were visualized in live L. mexicana promastigotes that expressed or were labeled with fluorescent markers, as follows. The ER is defined by a GFP chimera containing ...

The Late Secretory Pathway—from TGN to the Flagellar Pocket

In higher eukaryotes, the TGN is a major sorting station, where proteins destined for the cell surface are separated from those progressing to vacuolar and lysosomal compartments (366). Several lines of evidence suggest that the trans-most cisterna of the trypanosomatid Golgi is functionally equivalent to the TGN. First, the trans-most cisterna of the trypanosomatid Golgi is usually more highly dilated than earlier cisternae and is associated with a range of vesicular, cisternal, and multivesicular structures, suggestive of a sorting role (365). Second, cargo proteins such as VSG accumulate in this compartment when T. brucei BF are incubated at 20°C rather than 37°C (85). Third, the trans-cisterna can be selectively labeled with fluid-phase endocytic markers (176, 361, 365), suggesting that it is intimately connected to endocytic organelles by anterograde and retrograde transport vesicles (366). Finally, a number of protein markers, including a putative β1-adaptin (221) and reporter proteins containing a TGN targeting signal, termed the golgin-97, RanBP2α, Imh1p, and p230/golgin-245 (GRIP) domain, specifically localize to the trans-cisternae of T. brucei and L. mexicana Golgi (M. J. McConville, S. C. Ilgoutz, B. Foth, R. D. Teasdale, and P. A. Gleeson, submitted for publication), respectively, suggesting that it is a functionally distinct domain of the Golgi apparatus (Fig. (Fig.44).

The nature of the major transport intermediates that direct proteins from the Golgi to the flagellar pocket has yet to be precisely defined. In T. brucei BF, VSG is transported to the flagellar pocket in a complex system of cisternal and tubulo-vesicular membranes (85, 363). The unequivocal identification of these membranes as exocytic intermediates is complicated by the fact that VSG is also present in morphologically similar endosomal structures that are concentrated in the same region of the cell. However, some of these membranes are not labeled with fluid-phase endocytic markers and are thus likely to be primarily involved in exocytic transport (85, 363). In L. mexicana promastigotes, gp63 may be transported from the TGN to the flagellar pocket in large translucent vacuoles (226, 365). However, small transport vesicles are also commonly observed in the region between the Golgi apparatus and the flagellar pocket and may be involved in exocytosis. Thus, it is possible that transport to the flagellar pocket membrane involves a number of different carriers, possibly containing distinct proteins and lipid cargo, as has been found in other eukaryotes (136, 228, 267).

In some trypanosomatids, the lumen of the flagellar pocket may contain a gel-like matrix as well as many membrane profiles (176). In T. brucei BF, this matrix is rich in GPI proteins such as VSG and the transferrin receptor (119, 298, 338). The major GPI proteins of T. brucei procyclics and T. cruzi trypomastigotes are also abundantly present in the flagellar pocket lumen (119). It remains to be determined whether these membrane proteins are released into the lumen as micelles or as monomers. There is evidence that this matrix reduces the rate at which macromolecules diffuse out of the flagellar pocket (176).

Pathways from the TGN to Lysosomes and Vacuoles

Most trypanosomatid developmental stages contain at least two distinct classes of acidified vacuoles, the lysosomes and the acidocalcisomes (Fig. (Fig.3).3). The lysosomes are lytic vacuoles that receive material from the Golgi apparatus via a pleiomorphic population of endosome intermediates. The morphology of the lysosomes varies markedly in different trypanosomatid stages. In T. brucei BF and T. cruzi trypomastigotes, mature lysosomes comprise a series of prominent spherical vacuoles that characteristically have a perinuclear distribution (85, 176, 184, 332, 334, 374). In T. cruzi epimastigotes, the lysosomes (also termed reservosomes) contain electron-dense, lipid-rich cores and accumulate near the aflagellate end of the cell (270, 332) (Fig. (Fig.3).3). In rapidly dividing Leishmania promastigotes, the mature lysosomes exist as a highly unusual MVT, termed here the lysosome-MVT, that extends from the flagellar pocket to the posterior end of the cell (120, 226, 365) (Fig. (Fig.33 and and4).4). The Leishmania lysosome-MVT was first observed in live L. mexicana promastigotes expressing a GFP chimera of the ER glycosyltransferase, dolichol-phosphate-mannose synthase (DPMS), suggesting that it may have been part of the early secretory pathway (159). However, subsequent studies clearly demonstrate that it is a mature lysosome (120, 226, 365). In high-pressure-frozen and conventionally fixed L. mexicana promastigotes, the lysosome-MVT contains many small luminal vesicles and is clearly distinct from the ER and Golgi apparatus (120, 226, 365). This structure is highly reminiscent of late endosomes and lysosomes of other eukaryotes (126, 180). Moreover, the lysosome-MVT is the terminal compartment for a number of endocytic markers (FM 4-64, biotinylated surface proteins, and horseradish peroxidase) and is clearly distinct from the ER and Golgi apparatus. It also contains resident lysosomal proteases and is the site of degradation of several reporter proteins. Finally, glycoconjugates that are assembled in the Golgi apparatus can accumulate in the lysosome-MVT lumen, confirming that it is a post-Golgi compartment. Morphologically similar MVT structures occur in the related trypanosomatid Crithidia fasciculata (44) and in T. cruzi epimastigotes (270). However, the T. cruzi MVT is thought to correspond to a prelysosomal compartment and is termed here the late-endosome-MVT (Fig. (Fig.3).3). Interestingly, the L. mexicana lysosome-MVT matures into multiple electron-dense vacuoles as rapidly dividing promastigotes reach stationary growth (226, 265). In the amastigote stage, the lysosomes form large electron-dense vacuoles (termed megasomes) that occupy a significant proportion of the cytoplasm (63, 352). The morphology of late-endosome and mature-lysosome compartments can thus vary enormously within developmental stages of the same species. These developmental changes undoubtedly reflect the changing requirements for lysosomal degradation in regulating protein turnover and nutrient acquisition during the parasite life cycle.

Trypanosomatid proteins may be transported from the Golgi apparatus to the lysosomes via the flagellar pocket (the indirect route) or by a direct intracellular route (Fig. (Fig.5).5). While the ultrastructure of the endocytic membranes has been investigated in many trypanosomatids (see below), very little is known about the vesicular intermediates that deliver proteins to the lysosome from either the endosomes (indirect route) or the TGN (direct route). Putative vesicular intermediates have been identified in T. brucei (176, 184), Trypanosoma vivax (50), and Trypanosoma congolense BF (356). Recent studies with L. mexicana promastigotes have also identified a population of multivesicular bodies (MVBs) that form opposite the TGN and fuse with the lysosome-MVT (226). The involvement of MVBs in this step would be analogous to the recently delineated MVB pathway in yeast and animal cells (126, 180, 244, 283). MVBs are thought to form in the endocytic pathway by a process that involves the invagination of microvesicles from the outer membrane of endosomes that pinch off to form discrete structures in the MVB lumen. When MVBs fuse with the lysosome, these internal vesicles are delivered into the lysosome lumen and eventually degraded by soluble hydrolases (proteases, lipases, and glycosidases). Proteins and lipids destined for degradation are incorporated into the internal vesicles of the MVBs, whereas proteins that function at the lysosome surface remain in the MVB limiting membrane and can be recycled back to the early endosomes or the TGN (180). Several recent observations suggest that the MVBs in Leishmania and other trypanosomatids play a similar role. In particular, ER proteins such as DPMS (an integral membrane protein that is oriented on the cytoplasmic leaflet of the ER) are sorted into the lumen of the MVB and lysosome-MVT of stationary-phase L. mexicana promastigotes (226). Some peripheral leishmanial membrane proteins that associate with phosphoinositide lipids on the cytoplasmic leaflet of the endosomes are also delivered into the lumen of the lysosome (J. Callaghan and M. J. McConville, unpublished results). However, not all proteins are packaged into these lumen vesicles. For example, the T. brucei type 1 membrane proteins tGLP-1 and p67 are distributed between the Golgi apparatus and the limiting membrane of the lysosome in T. brucei BF (184). This distribution suggests that some proteins may undergo multiple cycles of transport between the Golgi apparatus to the limiting membrane of the lysosome (Fig. (Fig.5).5). Retrograde transport of proteins out of the lysosome is supported by the observation that proteolytically processed forms of p67 can be detected at the cell surface of T. brucei BF (41).

FIG. 5.
Proposed protein transport pathways in the secretory and endocytic pathways of trypanosomatids. Proteins are synthesized in the rough ER, comprising domains of the nuclear envelope (NE) and the cortical ER (ER), and then exported to the Golgi apparatus ...

Retrograde transport from the lysosome is likely to be important in recycling trypanosomatid flagellar pocket receptors. For example, the transferrin and lipoprotein receptors of T. brucei BF appear to be transported to either a prelysosome or mature lysosome compartment, where their ligands are released and degraded (186, 339). However, the receptors themselves are not degraded but are apparently recycled back to the flagellar pocket for further rounds of transferrin and lipoprotein uptake and internalization (339). This contrasts with the situation in animal cells, where the transferrin receptor recycles between the plasma membrane and a population of early endosomes. In this case the transferrin remains bound to the human transferrin receptor throughout the cycle (iron is released from the diferric [holo]transferrin-receptor complex in the early endosomes) and the iron-free (apo)transferrin is released only once the complex returns to the cell surface (350). After being delivered to the lysosome of T. brucei BF, the transferrin degradation products are secreted into the extracellular milieu (339). Similarly, the degradation products of antibodies internalized to the lysosome with other flagellar pocket receptors are also secreted (186). These observations indicate that the contents of the lysosome as well as lysosomal membrane proteins can be delivered back to the plasma membrane (Fig. (Fig.5).5). Delivery to the plasma membrane could occur via a retrograde pathway or by direct fusion of lysosomes with the flagellar pocket membrane (12).

The acidocalcisomes constitute the second class of acidified vacuoles in trypanosomatids (reviewed in reference 79). Similar vacuoles (also known as volutin granules or polyphosphate bodies) are present in apicomplexan parasites and some green algae (292). Unlike the lysosomes, the acidocalcisomes lack proteinase activities and appear to be storage organelles containing the major cellular reserves for phosphorus (mainly as polyphosphates), calcium, sodium, and a number of other cations (Zn2+ and Mg2+) (79, 80). They may also play a role in protecting these unicellular eukaryotes from osmotic stress (293). The acidocalcisomes appear to be empty by conventional electron microscopy but have a high electron density when cells are prepared without fixation and dehydration (79). They can be detected by fluorescence microscopy in living parasites that have been stained with acidotrophic or cationic dyes (acridine orange, Lysotracker, or DAPI [4′,6′-diamidino-2-phenylindole]) (226, 293). The intracellular distribution of acidocalcisomes varies in different developmental stages, alternatively clustering near the flagellum (T. cruzi trypomastigotes), the cell periphery (T. cruzi amastigotes), or the aflagellate end of the parasite (L. mexicana promastigotes) (79, 226). They can also be closely associated with other intracellular organelles, such as the ER and mitochondria, consistent with their being the dynamic storage reservoirs of Ca2+ and phosphate (217). These vacuoles are not labeled with endocytic markers in rapidly dividing trypanosomatid stages, suggesting that the lysosomes or earlier endocytic compartments do not fuse with the acidocalcisomes (217, 226, 313). However, in drug-treated parasites, endocytic markers can be internalized into acidocalcisomes (353), possibly as a result of nonselective autophagic degradation of intracellular organelles under these conditions. The limiting membrane of the trypanosomatid acidocalcisomes contains a V-H+ pyrophosphatase, a Na+/H+ exchanger, a Ca2+-H+ exchanger, a Ca2+-ATPase, and a V-H+-ATPase that maintain the acidic pH and concentrate various cations in the lumen (79, 311, 312). Resident proteins such as the V-H+ pyrophosphatase and V0 components of the V-H+-ATPase contain N-terminal signal sequences (143) and can also have dual localizations in the plasma membrane, suggesting that they are delivered to the acidocalcisomes via the Golgi apparatus or, alternatively, that the acidocalcisomes can fuse with the plasma membrane (293). Very little is known about the biogenesis of acidocalcisomes. A novel kinesin-like protein (TbKIFC1) that may associate with intermediates in acidocalcisome biogenesis and direct these structures along the subpellicular microtubules has recently been identified in T. brucei (87). Down-regulation of kinesin expression by double-stranded-RNA interference methods partially inhibited acidocalcisome function (87), although the effect of kinesin down-regulation on other post-Golgi compartments was not examined. These observations suggest that proteins are sorted into at least three distinct classes of transport vesicles in the Golgi apparatus that are targeted to the flagellar pocket, the endosome-lysosome system, and the acidocalcisomes.

Intersection of Secretory and Endocytic Pathways

Parasite survival within insect and vertebrate hosts is dependent on the uptake of extracellular nutrients and the removal of opsonic host proteins from the cell surface. Endocytosis in trypanosomatids is restricted to either the flagellar pocket membrane or, where present, the cytostome. The early endosomes commonly consist of a system of pleiomorphic tubules and cisternal structures that are invariably localized around the flagellar pocket and in close proximity to the Golgi apparatus (176, 361, 362, 365) (Fig. (Fig.3).3). However, the rate of endocytosis varies enormously in different trypanosomatids. In T. brucei BF, the entire flagellar pocket volume may be endocytosed six to eight times per h, equivalent to the internalization of the flagellar pocket membrane every 2 min (65). Endocytosis is mediated primarily by a population of clathrin-coated vesicles that bud from the flagellar pocket and deliver a range of fluid-phase markers (i.e., ferritin, horseradish peroxidase, fluorescein isothiocyanate-bovine serum albumin, gold-labeled bovine serum albumin, and lucifer yellow) and membrane markers (VSG and transferrin-, low-density lipoprotein-, and high-density lipoprotein-receptor complexes) to a system of cisternal elements and collecting tubules (176, 221). This tubule-vesicle complex contains distinct populations of endosomes, as defined by the distribution of several Rab protein homologues (TbRab4, TbRab5A, TbRab5B, and TbRab11) (104), which are likely to be active in sorting membrane and soluble components for transport to the lysosomes or back to the flagellar pocket. Compartments defined by TbRab4, -5A, and -5B are associated with endosomes that are involved in the internalization steps and possibly transport to late-endosome and lysosome compartments (104). In contrast, TbRab11 delineates a distinct population of endosome membranes that are closely associated with these compartments but which appear to be involved in recycling GPI proteins, such as the VSG and transferrin receptor, to the cell surface (163). Unexpectedly, some of these Rab proteins can be detected at the aflagellate end of T. brucei BF, raising the possibility that they may be involved in long-distance transport (104, 221). In T. brucei procyclics and most other trypanosomatids, the rate of endocytosis is much lower, although uptake of plasma membrane markers can still be readily detected (94, 120, 176, 178, 226, 362), and the morphology of the endocytic organelles is considerably less complex (106, 163, 221, 362, 365). The lower rate of endocytosis may reflect the absence of clathrin-coated endocytic vesicles in these developmental stages (176, 221). However, endocytosis is significantly increased in T. brucei procyclics overexpressing constitutively active forms of TbRab5A, suggesting that these vesicles can sustain a high level of endocytosis (251a).

Plasma membrane proteins and flagellar pocket receptors that are internalized into the tubular-vesicular endosomes may be recycled back to the flagellar pocket or transported to the late-endosome and lysosome compartments (43, 85, 132, 323, 361) (Fig. (Fig.5).5). Transport from the tubular-vesicular (early) endosomes to the lysosome is specifically inhibited when T. brucei BF and Leishmania promastigotes are incubated at 10 to 12°C (43, 132, 226), suggesting that this step is more temperature sensitive than the recycling step. By analogy with the situation in other eukaryotes (180), transport from the endosomes to the lysosomes may involve the late-endosome-MVB pathway described above. These organelles would thus represent the point at which the endocytic and secretory pathways converge (Fig. (Fig.5).5). Interestingly, the GPI proteins of trypanosomatids can also be internalized into the lysosome, along with other flagellar pocket receptors. Overath and colleagues estimated that approximately 25% of L. mexicana gp63 accumulates in the lysosome-MVT of the promastigote stage (365). A significant steady-state pool of GPI-anchored PPG is also present in these organelles (E. Handman, A. Piani, J. Curtis, T. Ilg, M. J. McConville, and B. Foth, submitted for publication). In another interesting series of studies, anti-VSG antibodies opsonized to the cell surface of T. brucei BF were found to be rapidly endocytosed into the endocytic pathway and delivered to perinuclear lysosomes (318, 364). Removal of a single layer of bound antibody was complete within 30 min under physiological conditions. As both bi- and monovalent antibodies and antibody fragments are internalized, it is likely that VSG is constitutively endocytosed at a very high rate and bound antibodies are subsequently degraded in the lysosome. However, it remains unclear whether all the endocytosed VSG reaches late-endosome and lysosome compartments or whether only opsonized VSG is diverted to these compartments. VSG is subsequently recycled back to the flagellar pocket in Rab11-positive endosomes (163). The internalization of VSG into late-endocytic compartments is likely to play a key role in preventing the accumulation of opsonic antibody on the surface coat of T. brucei BF (18, 242, 318, 364) and may provide a rationale for why the rate of endocytosis in this developmental stage is massively up-regulated compared to that in other trypanosomatids.

Endocytosis via the Cytostome

Some trypanosomatids contain a second specialized invagination in their plasma membranes, termed a cytostome, that constitutes an alternative site of endocytosis. Cytostomes are absent from T. brucei and Leishmania but are prominent in T. cruzi epimastigotes and amastigotes (Fig. (Fig.3).3). The cytostome of T. cruzi epimastigotes is located near the flagellar pocket and extends into the cytoplasm as a narrow tubule (the cytopharynx) with an acidified lumen (270, 334). Lectin binding and freeze fracture studies demonstrate that the plasma membrane around the cytostome and in the region between the cytostome and the flagellar pocket is distinct from the rest of the plasma membrane and that these structures overlie a set of specialized microtubules (332). Uncoated vesicles bud from the end of the cytopharynx and fuse with an MVT that extends along the anterior-posterior axis of the cell (270) (Fig. (Fig.3).3). Although this organelle is morphologically similar to the lysosome-MVT of L. mexicana promastigotes, it appears to be an intermediate compartment in the delivery of endocytic markers to a population of electron-dense lysosomes (reservosomes) at the posterior end of the cell (270) (Fig. (Fig.3).3). The structure of the cytostome and endocytic organelles has also been studied in C. fasciculata. In this case, the cytostome is located inside the flagellar pocket, and endocytic vesicles that bud from this structure deliver their contents to a series of MVBs that arise near the Golgi and subsequently fuse with an MVT reminiscent of that found in L. mexicana (44). Collectively, these studies demonstrate that the cytostome, rather than the flagellar pocket, is the major site of endocytosis in these trypanosomatids and that endocytosed material is delivered to terminal lysosomes via MVBs or MVT structures (44, 247, 270, 332, 334). It remains to be determined whether the cytostome is also involved in exocytosis and the role of the endosomes in the cytostome-lysosome pathway.

Components of the Vesicle Transport Machinery

In other eukaryotes, the fusion of transport vesicles with their target membrane is regulated by proteins of the soluble NSF attachment proteins (SNAP) receptor (SNARE) family (236). A v-SNARE on the vesicle interacts with a t-SNARE on the target organelle, and their interaction is required for membrane fusion. The fusion reaction and subsequent recycling of the SNAREs is regulated by soluble proteins, such as N-ethylmaleimide-sensitive factor (NSF) and SNAP, as well as a number of other proteins, including Rab GTPases and Sec1-like proteins (336). Analyses of the trypanosomatid genomes have identified 11 putative homologues of different Rab proteins, seven of which have been implicated in different mammalian membrane trafficking steps (Table (Table2).2). In contrast, only two SNARE proteins could be reliably identified based on sequence homology (unpublished observation). This result is likely to reflect the degree of conservation of these proteins across species. Comparison of functional homologues of these proteins between yeast and mammals shows that the Rab GTPases have a higher level of conservation than the SNARE proteins. The identification of additional SNAREs will require biochemical studies or the use of more sensitive sequence homology searches.

Putative homologues of membrane trafficking proteins identified in the genomes of T. brucei and L. major

A homologue of NSF and another member of the AAA (ATPase associated with different cellular activities) family of proteins, p97/cdc48p, have been identified in T. brucei (289) (Table (Table2).2). These proteins are thought to be responsible for unraveling highly stable SNARE complexes and thus play a key role in priming or recycling SNAREs for the next round of vesicle fusion. While NSF acts in most vesicle transport steps, p97 is thought to be involved in regulating the homotypic fusion of ER and Golgi membranes and the biogenesis of these organelles. The T. brucei p97 gene complements the yeast cdc48 gene, encodes a protein that forms hexameric complexes, and contains two functional ATPase domains (173, 289). This protein is essential for parasite growth, and the regulated expression of dominant negative forms (in which one of the ATPase domains is mutated) results in gross changes in cell shape (173). However, it does not appear to play a direct role in exocytosis of soluble or GPI proteins, and its potential function in regulating organellar division remains to be determined.

In addition to the membrane targeting and fusion machinery, a number of coat protein complexes drive the initial formation of a membrane vesicle and also play a key role in selecting protein cargo and cargo receptors (336). Vesicle formation requires the recruitment of the coat proteins from the cytosol either as individual proteins or as preformed complexes. Following vesicle formation, the coat proteins are released, allowing the SNAREs and other tethering proteins to interact with their counter receptors. Well-characterized coat proteins include clathrin and the adaptor 1 and 2 complexes (Golgi-to-plasma membrane and plasma membrane-to-early-endosome transport, respectively), COPI (Golgi-to-ER and intra-Golgi transport), and COPII (ER-to-Golgi transport) (336). Additional coat proteins are thought to be involved in regulating the transport of TGN tubular vesicles to the plasma membrane and retrograde transport from the endosomes to the TGN (180, 314). Open reading frames that encode putative homologues of many of these coat proteins are present in the T. brucei and L. major genome databases (Table (Table2).2). In T. brucei BF, endocytosis is largely mediated by coated vesicles that contain clathrin heavy chain (221, 320). Potential adaptor proteins and an α-dynamin homologue that may facilitate this process are present in the databases (Table (Table2).2). Expression of the T. brucei clathrin heavy chain is markedly up-regulated in the BF stage compared to the procyclic stage, consistent with the finding that the endocytic vesicles with a conspicuous cytoplasmic coat are absent in the latter stage (176, 221, 361). The nature of the cytoplasmic coat on these endocytic vesicles remains to be determined. Clathrin-coated vesicles may also mediate transport between the Golgi apparatus and the endosomes in T. brucei BF, as suggested by the partial distribution of the clathrin heavy chain to the Golgi region and the identification of a putative β1-adaptin homologue (221). Unlike the clathrin heavy chain, β1-adaptin was expressed at similar levels in both T. brucei BF and procyclics, indicating that this pathway is similarly active in both stages (221). Protein coats have also been observed on post-Golgi vesicles in L. mexicana promastigotes (365). Finally, putative homologues of COPII and COPI coat complexes have been identified in the trypanosome and leishmania genomes (Table (Table2),2), and a high-molecular-weight COPI complex has been partially purified from T. brucei procyclics (195). Interestingly, secretory transport in T. brucei, T. cruzi, and Leishmania is not inhibited by brefeldin A, a potent inhibitor of COPI coat formation in many animal and protozoan cells (93, 108) (Mullin and McConville, unpublished), suggesting that one or more proteins involved in ER-Golgi transport in trypanosomatids differ from their mammalian counterparts. Overall, trypanosomatids have numerous proteins encoded in their genomes related to proteins that function in the various membrane trafficking stages in both yeast and mammalian cells. Based on the range of proteins identified, trypanosomatids would be predicted to have the same membrane transport pathways, utilizing similar protein machinery, to those already identified in other eukaryotes.

Role of the Microtubule Cytoskeleton

Microtubules are the major cytoskeletal elements of trypanosomatids (reviewed in reference 127). There is increasing evidence that the subpellicular microtubules that underlie the plasma membrane, as well as a limited number of specialized transcellular microtubules, may play a role in regulating the polarized distribution and biogenesis of secretory and endocytic pathway organelles. They may do this in two ways: by sterically restricting exo- and endocytic functions to certain plasma membrane domains and/or by acting as cytoplasmic scaffolds for specific organelles or transport intermediates.

The subpellicular array comprises more than 100 microtubules that are aligned along the anterior-posterior axis of the cell and are highly cross-linked both to each other and to the overlying plasma membrane. Microtubule attachment to the plasma membrane may be mediated by acylated microtubule-binding proteins (142, 305) or polytopic integral membrane proteins (331). It is generally assumed that the subpellicular microtubules limit the accessibility of vesicular traffic to all domains of the plasma membrane except the flagellar pocket (and cytostome, where it exists) and thus impose a degree of polarization on the distribution of secretory and endocytic organelles. However, large secretory granules can reach the plasma membranes of other protozoan parasites that contain a highly organized cortical (membrane or microtubule) skeleton (235), and some domains of the ER can clearly penetrate between the subpellicular microtubules in trypanosomatids (264). These indirect lines of evidence raise the possibilities that the subpellicular microtubules may play a more active role in directing vesicular traffic to the flagellar pocket and/or that specific protein or lipid determinants on the flagellar pocket membrane act as targeting signals. In support of an active role for the subpellicular microtubules, a number of microtubule-binding proteins have recently been identified that are directed to different ends of these microtubule arrays and may function as motor proteins. For example, a GFP chimera containing the microtubule-binding protein trypanin (previously called T-lymphocyte-triggering factor) accumulates at the posterior face of the flagellar pocket of T. brucei BF. Remarkably, a GFP fusion containing the mammalian homologue of trypanin accumulates at the extreme posterior end of the trypomastigotes, where the subpellicular microtubules terminate (144, 145). The T. brucei and mammalian proteins may bind to different motor proteins and/or different microtubules within the subpellicular array. In particular, the localization of the T. brucei GFP-trypanin chimera suggests that it might bind to the microtubule quartet, a specialized set of four microtubules that underlie the FAZ. These microtubules arise near the flagellum basal body before being intercalated into the subpellicular array, have the polarity opposite to that of other subpellicular microtubules, contain γ-tubulin, and are more resistant to high-salt extraction than the subpellicular microtubules (286, 294, 372). The possible involvement of the FAZ microtubules in organelle positioning is supported by the tight association of ER subdomains with these microtubules along part of their length (357). Finally, a kinesin-like motor protein that binds to microtubules in vitro and membrane-bound organelles that may be required for the biogenesis of mature acidocalcisomes in vivo has been identified in T. brucei (87). In the presence of NH4Cl, these structures move to the minus end of subpellicular microtubules, suggesting that such movement is dependent on intracellular pH gradients.

While the studies described above suggest that the subpellicular microtubules may play a role in directing membrane transport, most organelles in the trypanosomatid secretory and endocytic pathways are not associated with the subpellicular array. However, there is evidence that in C. fasciculata and Leishmania promastigotes, the subcellular positions of some of these organelles, including the Golgi apparatus and the lysosome-MVT, may be maintained by one or two cytoplasmic microtubules that extend along the anterior-posterior axis of the parasite (44, 220, 226, 365). Whether these cytoplasmic microtubules are related to or are the same as the microtubule quartet of T. brucei and T. cruzi trypomastigotes is not known. Compounds that disrupt intracellular pH gradients cause the rapid collapse of the lysosome-MVT, possibly as a result of the dissociation of these labile membranes from these microtubules (159, 226). These microtubules may also have a role in segregating the Golgi apparatus and populations of endosomes into daughter cells during mitosis, as this processes is tightly coordinated with the division of the basal body (105, 163).


Surface Transport of GPI-Anchored Glycoproteins

The major surface proteins of trypanosomatids are initially synthesized with a cleavable N-terminal signal sequence and a C-terminal GPI attachment signal that is rapidly replaced (within 1 min) with a GPI anchor in the ER lumen (10, 20, 22, 23, 68, 97, 182, 198, 226). After addition of the GPI anchor, these proteins are transported to the cell surface with comparatively rapid kinetics. For example, VSG is transported to the surface of T. brucei BF with a half time (t1/2) of approximately 15 min (20, 85), while gp63 is transported to the surface of L. mexicana promastigotes with a t1/2 of 40 min (280). If anchor addition is prevented, by either deletion of the GPI transamidase (146) or depletion of GPI anchor precursors 116, 214, 230; M. Ellis, J. D. Hilley, D. K. Sharma, S. Lillico, G. H. Coombs, and J. C. Mottram, Mol. Parasitol. Meet. XI, abstr. 135, 2000), the newly synthesized proteins are either slowly secreted or degraded. The rapid surface transport kinetics of VSG and gp63 raises the possibility that these proteins may be selectively incorporated into ER transport vesicles and exported at a rate that is higher than bulk flow. Efficient export from the ER is supported by immunoelectron microscopy studies showing that steady-state levels of VSG and gp63 in the ER are very low, despite the fact that these proteins are synthesized at very high rates in metabolic labeling experiments (97, 365). Second, VSG is transported to the cell surface of T. brucei BF with faster kinetics than that of the integral membrane protein, p67 (t1/2, 15 versus ~60 min) (41). Third, Bangs and colleagues have shown that GPI-anchored VSG is transported to the plasma membrane with faster kinetics than a soluble form of VSG (lacking a GPI signal sequence) when these proteins are ectopically expressed in T. brucei procyclic stages (t1/2, ~1 versus 5 h) (24, 207). Moreover, the soluble forms of VSG accumulate in the ER, suggesting that the addition of a GPI anchor is required for efficient export via the tER. Finally, gp63 is transported to the surface of L. mexicana promastigotes with faster kinetics (twofold) than the more abundant free GPIs, which may be transported by bulk flow (280).

Recent studies with yeast suggest that the major GPI protein of Saccharomyces cerevisiae, Gas1p, is selectively incorporated into a subpopulation of COPII-coated ER transport vesicles and that this transport step is dependent on COPI coat components and ongoing ceramide synthesis (82, 148, 227, 344). Two models, which are not mutually exclusive, have been proposed to account for the selective recruitment of GPI proteins into these ER vesicles (228). The first of these models posits that Gas1p is recognized by the p24 family of cargo receptors (169, 227). Homologues of these proteins have been identified in the T. brucei genome (194; R. D. Teasdale and M. J. McConville, unpublished data) and may selectively recognize partially conserved features in the VSG polypeptide or the GPI moiety itself. It is worth noting that some conformational epitopes in VSG are lost upon removal of the GPI anchor (52), possibly accounting for the slower transport of nonanchored forms of VSG that may no longer be recognized by an ER receptor. The presence of putative cargo receptors in the tER may also explain why gp63 is transported to the cell surface with faster kinetics than the free GPIs of L. mexicana (Ralton et al., submitted) and why many foreign proteins get trapped in the ER when ectopically expressed in T. brucei BF (U. Bohme, E. Wirtz, M. Duszenko, and G. A. M. Cross, Mol. Parasitol. Meet. X, abstr. 201, 1999). In the second model, the efficient export of Gas1p from the ER of yeast reflects the association of this protein with sphingolipid-rich membranes or rafts in the ER that are subsequently incorporated into COPII vesicles (15). In support of this model, anterograde transport of yeast Gas1p, but not integral membrane proteins, requires ongoing sphingolipid biosynthesis (148, 344). However, more recent studies have shown that the major raft-forming sphingolipid of yeast is made in the Golgi apparatus rather than the ER (181) and that sphingolipids are also required for fusion of ER vesicles with the Golgi (344). Finally, inhibitors of sphingolipid biosynthesis do not affect the rate of surface transport of gp63 in L. mexicana promastigotes (280). It is therefore likely that the forward transport of GPI proteins in Leishmania does not involve a lipid-based sorting mechanism and that the requirements for surface transport of GPI proteins in yeast and trypanosomatids are different.

Several recent studies suggest that the GPI anchors could also act as a cell surface sorting signal in the late secretory pathway of trypanosomatids. For example, when expressed at high levels, GPI proteins are efficiently transported to the cell surface while many integral membrane reporter proteins accumulate in the lysosome. Examples of integral membrane proteins that accumulate in the lysosome-MVT of Leishmania spp. when expressed at high levels include the membrane-bound acid phosphatase (normally found in endosomes) (365), a chimera of GFP containing the transmembrane domain of plasma membrane 3′-nucleotidase (120), and several GFP chimeras containing ER glycosyltransferases (226). Replacement of the transmembrane domains of the acid phosphatase and GFP with a GPI signal sequence results in the efficient expression of this protein at the cell surface. These studies raise the possibility that the lysosome is the default pathway for many integral membrane proteins, as is the case in yeast (62), and that addition of a GPI anchor redirects proteins into exocytic transport vesicles in the Golgi apparatus. Alternatively, GPI proteins may be sorted from integral membrane proteins in the flagellar pocket (41). In the latter case, addition of a GPI anchor may reduce the rate at which the protein is endocytosed or increase the efficiency with which it is recycled to the flagellar pocket. Interestingly, L. mexicana promastigotes express a number of different isoforms of gp63 that all contain a GPI attachment signal and are targeted predominantly to the cell surface. In contrast, the amastigote stage expresses a single isoform of gp63 that lacks a GPI attachment signal (but contains a C-terminal hydrophobic domain) and is localized to the lysosome (16). Thus, the stage-specific expression of protein isoforms with or without a GPI attachment signal may lead to the redistribution of the same protein to the plasma membrane or the lysosome.

The sorting of heterologous GPI proteins to the plasma membrane is likely to involve a lipid-based sorting mechanism. In this respect, a number of recent studies have shown that trypanosomatid GPI proteins become associated with detergent-resistant membranes (DRMs) during transit to the cell surface (73, 238, 280). DRMs have been found in all eukaryotes that have been investigated and are thought to correspond to dynamic micro- or macrodomains in intracellular and plasma membranes that are present largely in a liquid-ordered, rather than a liquid-disordered (fluid), state (46, 47). In common with the DRMs of other eukaryotes, the Leishmania promastigote DRMs are highly enriched in sphingolipids (inositolphosphoceramide), sterols (primarily ergosterol), and GPI proteins and free GPIs. They have a light buoyant density in sucrose density gradients and are depleted of integral membrane proteins (73, 280). Interestingly, newly synthesized gp63 is incorporated into DRMs upon arrival at the cell surface of L. mexicana promastigotes but at a much earlier point in L. major promastigotes (73, 280), suggesting that the lipid composition of secretory pathway membranes varies between species. More strikingly, DRMs can be detected in T. brucei only when these parasites are extracted in dilute (0.5 rather than 1%) Triton X-100 (73, 237). Thus, if DRMs do act as sorting platforms in the late secretory pathway of trypanosomatids, they are unlikely to have a specific lipid composition.

Surface Transport of Integral Membrane Proteins

The plasma membranes of trypanosomatids also contain a number of functionally diverse type 1 and polytopic membrane proteins (Table (Table1).1). These proteins may contain sorting signals that prevent them from being transported to the lysosome. In the case of L. donovani 3′-nucleotidase, this putative sorting signal may reside in the luminal domain as the full-length protein is efficiently transported to the plasma membrane even when overexpressed (68), while GFP chimeras containing the transmembrane and cytoplasmic domains of 3′-nucleotidase are primarily transported to the lysosome-MVT (120).

Other studies have provided evidence that efficient export of some integral membrane proteins from the ER is signal mediated. Deletion of 19 amino acids from the cytoplasmic tail of the T. brucei high-density lipoprotein receptor (cysteine-rich repetitive acidic transmembrane protein [CRAM]) results in the accumulation of the mutated protein in the ER (375). However, further studies are needed to discount the possibility that ER retention is not due to a defect in the folding of this protein.

Sorting in the Flagellar Pocket

The flagellar pocket appears to constitute an important sorting compartment in its own right. While the major GPI proteins and surface transporters are swept out of the flagellar pocket to the cell body and/or the flagellum, a number of cell surface receptors and resident lysosomal proteins are retained within the flagellar pocket and enter the endocytic recycling and/or lysosomal transport pathways. Recent studies suggest that sorting signals may be present in both the cytoplasmic tails and luminal domains of flagellar pocket proteins. In the case of the high-density lipoprotein receptor, CRAM, sequences in the cytosolic tail of this protein (near the transmembrane domain) are both necessary and sufficient for the steady-state localization of CRAM and a reporter protein to the flagellar pocket of T. brucei procyclics (375). This domain is also required for the endocytosis and transport of CRAM to the lysosome (186). Thus, the flagellar pocket localization of CRAM in T. brucei procyclics could reflect the continuous internalization of this receptor into the endosome-lysosome system and recycling back to the flagellar pocket.

In contrast, the T. brucei BF transferrin receptor is a heterodimer of ESAG-6 (a GPI protein) and ESAG-7 (a highly related protein lacking a GPI signal) and thus lacks a cytoplasmic polypeptide domain (183, 298, 337). The retention and internalization signals in the receptor must therefore reside in either the luminal or GPI domains of these proteins. Nolan and colleagues recently proposed that endocytosis of a number of flagellar pocket receptors and lysosomal proteins in T. brucei BF is regulated by a lectin-like receptor that binds to luminally oriented N-linked glycans on these proteins (237). This hypothesis is based on the finding that several of these receptors (including the transferrin receptor, ISG100, p67/CB1-gp, and ESAG-2) are strongly recognized by the tomato lectin that binds branched poly-NAL glycans and that the uptake of transferrin is inhibited by GlcNAc-containing oligosaccharides (237). Furthermore, when the dimeric ESAG-6 and -7 receptor complex is expressed in T. brucei procyclics, these proteins are modified with high-mannose N-glycans and are distributed over the entire cell body (183). However, direct evidence for a poly-NAL receptor has yet to be obtained, and it remains to be determined how such a mechanism could work given that the flagellar pocket will also contain very high levels of VSG with similar poly-NAL chains. If a lectin receptor does exist, it is likely to be restricted to T. brucei BF, as this is the only trypanosomatid to synthesize poly-NAL N-glycans (see below).

Some surface proteins, such as the glucose transporters of Leishmania enriettii, are sorted to either the cell body plasma membrane or the flagellum (174). Glucose transporter isoform 2 is directed to the cell body by a short N-terminal cytoplasmic tail that mediates the attachment of this protein to the subpellicular microtubules that underlie the cell body (331). On the other hand, glucose transporter isoform 1 has a longer (139-amino-acid) cytoplasmic domain that contains a flagellar-membrane-targeting motif (266, 330, 331). From alanine-scanning mutagenesis, this targeting motif was restricted to five contiguous amino acids. Furthermore, it was proposed that flagellum localization may be mediated by continuous recycling of the isoform 2 transporter between the flagellum and the flagellar pocket. It will be of interest to determine whether these proteins associate with cytoplasmic raft complexes that have been shown to move up and down the flagellum via interactions with flagellar microtubules and motor proteins in other protists (260). A number of other proteins have been localized to the flagellum of other trypanosomatids, including the receptor adenylate cyclase (ESAG-4) from T. brucei and the cytosolically oriented Ca2+-binding proteins of T. brucei and T. cruzi (122). These proteins lack the cytoplasmic peptide motifs of the leishmanial transporters and appear to be targeted to the flagellum by additional mechanisms.

Sorting in the Endosomes

Only a few protein markers for the trypanosomatid endosomes have been identified. These include a number of Rab proteins (Table (Table2)2) (106), the membrane-bound acid phosphatase of L. mexicana promastigotes (367), and the Leishmania tarentolae ABC transporter, glycoprotein-like protein A (PGPA) (179). Overexpression of the L. mexicana membrane-bound acid phosphatase in wild-type cells results in the transport of this protein to the cell surface and the lysosome-MVT (365). The endosomal localization of this protein may thus depend on saturable endocytic and recycling steps. As a truncation mutant of the acid phosphatase comprising only the luminal domain is secreted, this signal(s) must reside in the cytoplasmic or transmembrane domains of this protein (367).

Targeting of Lysosomal Proteins

Most newly synthesized lysosomal hydrolases and integral membrane proteins are delivered to the trypanosomatid lysosomes via the secretory pathway. This is supported by the following findings. First, most resident lysosomal proteins characterized to date contain a canonical N-terminal signal sequence that directs nascent polypeptides into the lumen of the ER (150, 167). Second, these proteins are modified with N-glycans and terminal carbohydrate modifications that occur only in the ER and Golgi lumens, respectively (41, 55, 255). Third, unprocessed lysosomal proteases accumulate in the Golgi or flagellar pocket (45, 93). Finally, inhibition of these processing steps with protease inhibitors results in dramatic changes in Golgi structure (93). Transport of proteins to the lysosomes of trypanosomatids may occur via two routes, the direct intracellular pathway from the Golgi apparatus to the lysosomes, most likely via an endosome intermediate (see above), and the indirect surface pathway, where proteins are first transported to the flagellar pocket before being transported to the lysosome via the endocytic pathway (Fig. (Fig.5).5). The extent to which some proteins are transported along one or the both of these pathways is developmentally regulated (168).

Cysteine proteases.

The cysteine proteases are a major class of soluble lysosomal hydrolases in all trypanosomatids. These proteinases are initially synthesized as prepropolypeptides with an N-terminal signal peptide, a 100- to 122-amino-acid proregion, a central catalytic domain, and, in some cases, an unusual 100-amino-acid C-terminal extension (55, 150). The N-terminal propeptide is thought to maintain these enzymes in an inactive state and to facilitate folding in the ER. The propeptide is also required for lysosomal targeting of cruzain (the major cysteine protease of T. cruzi) and is capable of directing reporter proteins such as GFP to lysosomes in both T. cruzi and Leishmania (150). These studies suggest that the prodomain is recognized by an unidentified receptor in the early secretory pathway and proteolytically removed during transit to or upon arrival in the lysosome. If cleavage of the cruzain propeptide is inhibited, by either expression of forms with a mutated cleavage site or incubation of T. cruzi epimastigotes in cysteine protease inhibitors (150), the propeptide accumulates in the Golgi apparatus rather than being secreted. Prolonged treatment of T. cruzi epimastigotes with cysteine protease inhibitors induces dramatic changes in structure of the Golgi apparatus as well as the ER (84, 93, 315), possibly accounting for the toxicity of these compounds to many trypanosomatids (92, 208, 315). These data suggest that the major cysteine proteases of T. cruzi epimastigotes are transported to the lysosomes via the direct intracellular route. In contrast, unprocessed cysteine proteases accumulate in the flagellar pocket of a protease-deficient L. mexicana mutant (45). It was concluded that these proteases normally transit via the flagellar pocket, although it remains possible that the flagellar pocket localization is due to the saturation of an intracellular cargo receptor. Interestingly, the prodomains of trypanosomatid cysteine proteases contain a nine-residue domain that shares close homology with a related domain in mammalian procathepsin L. This domain is apparently required for lysosomal traffic via a mannose-6-phosphate-independent pathway. As there is no evidence that trypanosomatids contain a mannose-6-phosphate pathway (45, 84), these parasites may constitute an interesting model system for investigating lysosomal targeting mechanisms that may have been conserved throughout eukaryotic evolution (150). Finally, there is evidence that some fully processed cysteine proteases are secreted (84, 246). The secretion of these proteases may represent the saturation of cargo receptors in the secretory pathway or the exocytosis of lysosomal contents (12).

Lysosomal membrane proteins.

The paradigm for lysosomal membrane protein transport in trypanosomatids is the T. brucei type 1 membrane glycoprotein, p67, which has a domain structure similar to that of the lysosomal acidic membrane proteins of animal cells (167). In T. brucei BF, newly synthesized p67 is initially detected as a 100-kDa ER glycoform that is modified with 14 N-linked oligosaccharides. The N-glycans of p67 are extended and elaborated with a novel galactose-containing glycan (the CB1 epitope) in the Golgi apparatus to form the 150- to 180-kDa “Golgi” glycoform. This form is subsequently processed into smaller fragment by proteases in the endosome and lysosome compartments. By following these processing steps in conjunction with surface biotinylation, Brickman and Balber (41) and Kelley and colleagues (168) have shown that a significant fraction of p67 in T. brucei BF is transported from the Golgi apparatus to the flagellar pocket before being internalized via the endocytic pathway and delivered to lysosomes. Furthermore, processed forms of p67 can be detected at the plasma membrane, supporting the notion that some lysosomal proteins are transported back to the flagellar pocket (41). In contrast, T. brucei procyclics synthesize only an ER glycoform that is transported directly from the TGN to the lysosomes (168). p67 contains a number of potential targeting signals (dileucine and acidic amino acids) in its C-terminal cytoplasmic domain (167), and truncation mutants lacking this domain are transported to the cell surface of T. brucei procyclics (D. L. Alexander and J. D. Bangs, Mol. Parasitol. Meet., abstr. 59, 2000). The C-terminal domain is thus likely to play a role in sorting p67 in the Golgi apparatus into the lysosomal pathway.

Nonclassical Secretion

Most cell surface and secreted proteins are delivered to the plasma membrane via the secretory pathway. However, there is increasing evidence that alternative pathways exist in eukaryotic cells for secreting proteins which lack an N-terminal signal sequence but which contain alternative targeting signals. These so-called nonclassical secretory pathways include the regulated exocytosis of lysosomal compartments (i.e., interleukin 1β, basic fibroblast growth factor) (11, 12), the formation of exvaginating plasma membrane vesicles (i.e., galactin-1) (211), and the extrusion of polypeptides across internal or plasma membranes by polytopic ABC transporters (i.e., yeast a-factor). Recent studies on a family of hydrophilic acylated surface proteins (HASPs) from Leishmania spp. suggest that one or more of these pathways may also exist in trypanosomatids. The HASPs (previously called GBP and GA/CP) were initially detected in screens for genes that are selectively expressed on infective metacyclic promastigote and amastigote stages of Leishmania spp. The sequences of the HASP genes predict a family of hydrophilic proteins, 10 to 44 kDa in size, that lack an N-terminal signal sequence. In early studies, these proteins were found to be associated with either the entire cell body or the flagellar pocket (281), to be accessible to surface probes (i.e., biotinylation and surface antibodies), and to be hydrophobic proteins based on their tendency to partition into Triton X-114 detergent phases (326). Recent biochemical studies show that these proteins are N-terminally myristoylated and palmitoylated and that both modifications are required for surface expression (1, 74). An 18-amino-acid N-terminal peptide can direct the reporter protein GFP to the cell surface, while mutation of the single cysteine residue in this domain (the putative site of palmitoylation) resulted in the accumulation of the GFP in a compartment that was identified as the Golgi apparatus (74). A tentative model for secretion of the HASPs has been proposed in which these proteins are cotranslationally myristoylated before being transported to the cytoplasmic leaflet of the Golgi apparatus, where they are palmitoylated. The diacylated protein may then be translocated across the membrane of the Golgi apparatus or a post-Golgi compartment and secreted via the flagellar pocket. This process appears to be relatively inefficient (only 10 to 20% of HASPB can be detected at the cell surface), and nothing is known about the translocation mechanism. Remarkably, HASPB is also transported to the surface of CHO cells, suggesting that this pathway of nonclassical secretion has been broadly conserved during eukaryotic evolution. The extent to which other trypanosomatid proteins are secreted by this pathway is unknown. T. brucei GPI-phospholipase C (PLC) is generally considered a cytoplasmic protein, but recent studies suggest that it may access GPI-anchored proteins that are located in the lumen of the secretory pathway or on the cell surface (119). Like HSAPB, the T. brucei GPI-PLC lacks an N-terminal signal sequence and is multiply acylated (14, 256). Whether this enzyme is similarly translocated across intracellular or plasma membranes remains to be examined.



Assembly and processing of N-glycans in the ER

Most proteins in the secretory pathway of trypanosomatids are modified with N-linked glycans (252). As in other eukaryotes, these oligosaccharides are assembled on a dolichol lipid in the ER and are then transferred en bloc to newly synthesized proteins in the lumen of the ER. Work carried out by Parodi, Previato, and colleagues has established that the steps in dolichol-linked oligosaccharide biosynthesis are the same as in other eukaryotes (reviewed in reference 252). This pathway is initiated with the transfer of GlcNAc-1-PO4 from UDP-GlcNAc to dolichol phosphate to form GlcNAc-P-P-dolichol. The gene for the L. mexicana GlcNAc-1-phosphotransferase has been cloned (60) and localized to the bulk ER (K. A. Mullin, S. C. Ilgoutz, and M. J. McConville, unpublished observations). This enzyme is essential for growth of Leishmania (60) and has been used as a selectable marker in gene expression studies with the drug tunicamycin (187). The endogenous dolichols of T. brucei and Leishmania are shorter than those found in animal cells (containing 11 or 12 rather than ~20 five-carbon isoprene units) (188), but there is no evidence that the trypanosomatid GlcNAc-1-phosphotransferase selectively utilizes shorter dolichols in vitro. Subsequent steps in dolichol-linked oligosaccharide biosynthesis involve the addition of a second GlcNAc residue followed by six to nine mannose residues. In contrast to the situation in all other eukaryotes, none of the trypanosomatid dolichol-linked oligosaccharides are capped with glucose residues, as these parasites do not synthesize the sugar donor (dolichol-phosphate-glucose) for these reactions. Thus, most pathogenic trypanosomatids transfer Man9GlcNAc2 onto newly synthesized proteins (Fig. (Fig.6).6). Leishmania spp. also lack some of the dolichol-P-Man-dependent mannosyltransferases and transfer smaller Man6-7GlcNAc2 oligosaccharides to protein. Not surprisingly, the trypanosomatid oligosaccharidyltransferase complex shows little preference for glucosylated Man9GlcNAc2 oligosaccharides over the truncated versions in vitro (252). This is in contrast to the situation in yeast and mammalian cells, where the oligosaccharidyltransferase preferentially transfers glucosylated Man9GlcNAc2 structures to nascent proteins.

FIG. 6.FIG. 6.FIG. 6.
Secretory pathway modifications of proteins and GPIs in trypanosomatids. Species- and stage-specific differences in the assembly and processing of N-linked glycans, protein-linked and free GPIs, and O-linked glycans and phosphoglycosylation are highlighted. ...

Once dolichol-linked oligosaccharides are transferred to protein in the lumen of the ER, they are transiently modified with one or two glucose residues by a soluble UDP-Glc-dependent glucosyltransferase. These terminal glucose residues are subsequently removed by the concerted action of glucosidase I and II. This cycle of ER glucosylation and deglycosylation of N-linked glycans was first identified in trypanosomatids (facilitated by the fact that the parasites transfer nonglucosylated oligosaccharides to protein) but is now known to occur in many other eukaryotes (253, 254, 349). The glucosyltransferase is thought to recognize unfolded or misfolded proteins in the ER lumen. Glucosylated proteins subsequently interact with the lectin chaperones calnexin and calreticulin, which facilitate their folding and/or oligomerization. Trypanosomatids contain a calreticulin homologue, and the intracellular transport of T. cruzi lysosomal proteins is strongly impeded in the presence of glucosidase inhibitors (168, 171). Direct binding between T. cruzi calreticulin and a major lysosomal protease as also been demonstrated (172). On the other hand, inhibitors of N-glycosylation have little effect on the processing of Leishmania gp63 (110). Moreover, most of the mature N-glycans on gp63 and the secreted PPGs of L. mexicana retain one or more terminal glucose residues (157, 248), suggesting that the removal of these residues is not essential for glycoprotein export from the ER.

Golgi modifications of N-linked glycans

Further processing of N-linked glycans in the ER and Golgi apparatus is highly variable in different trypanosomatids (Fig. (Fig.6).6). Some trypanosomatid parasites that infect only insects or nonmammalian hosts contain N-linked glycans with highly unusual (i.e., ribose, rhamnose, or galactofuranose) terminal glycan modifications (215). In contrast, the N-glycans of secretory and lysosomal proteins in Leishmania, T. cruzi, and T. brucei procyclic stages undergo minimal modifications in the Golgi apparatus (Fig. (Fig.6).6). These high-mannose glycans may be trimmed by a soluble α1,2-mannosidase in the ER to generate mature glycans with the structures (+/-Glc)Man4-8GlcNAc2 (252). Although most N-linked glycans in these parasites are of the high-mannose type, many trypanosomatids retain the enzymatic machinery for making more complex N-glycan structures. For example, some lysosomal and surface proteins of T. cruzi (e.g., cruzain and Tc85) are modified with galactose-containing N-linked glycans (66, 255) (Fig. (Fig.6).6). Similarly, wild-type T. brucei procyclic stages bind galactose-binding lectins and concanavalin A-resistant mutants that cap the high-mannose glycans of the procyclins with the single N-acetyllactosamine unit, Galβ1-4GlcNAc, have been isolated (5, 151). In contrast, the major surface and lysosomal glycoproteins of T. brucei BF are elaborated with complex N-linked glycans, primarily biantennary glycans with branched and linear poly-NAL sequences, similar to those of higher eukaryotes (210, 376). Some of these glycans may be capped with the immunogenic Galα1-3Gal epitope, which is recognized by antibodies in human serum. These processing steps occur within several resolvable compartments in the Golgi apparatus (124). Lectin and antibody-binding studies suggest that the addition of these complex glycans is protein dependent, as some flagellar pocket receptors appear to contain distinct glycans (237). Not all the VSGs in T. brucei BF contain complex glycans. The mammalian cytokine tumor necrosis factor has been shown to bind to VSGs that retain a Man6-9GlcNAc2 N-linked glycan (193). Binding is restricted to the flagellar pocket, where these glycans appear to be more exposed, and the bound TNF is subsequently internalized into lysosomes (193).

Biosynthesis of GPI Protein Anchors

Assembly of intermediates in the ER.

GPI anchor precursors are assembled in the ER and subsequently transferred to newly synthesized proteins by a luminally oriented GPI transamidase (101, 204). The synthesis of GPI anchor precursors is highly up-regulated in T. brucei BF and procyclics, and these parasites have been used as model experimental systems to delineate the essential steps in GPI biosynthesis that have been conserved in all eukaryotes (100). All of the GPIs synthesized in T. brucei appear to be potential anchor precursors, although the rate of synthesis of these glycolipids is at least 10-fold higher than is required to sustain normal rates of VSG synthesis (279). The precise fate of these excess intermediates (whether they are metabolized or transported out of the ER) is unclear. GPI biosynthesis is essential for the growth of T. brucei BF in culture, possibly because the VSG coat stabilizes the plasma membrane or because of the essential role of other GPI proteins such as the transferrin receptor (230). In contrast, GPI protein anchor biosynthesis is not essential for growth of T. brucei procyclics (230) or for L. mexicana promastigotes and amastigotes (146). The major steps in the biosynthesis of T. brucei BF protein anchor precursors are shown in Fig. Fig.7,7, while the enzymology of these reactions has been comprehensively reviewed in reference 101. Protein anchor biosynthesis involves (i) the addition of GlcNAc to phosphatidylinositol (PI) and subsequent de-N-acetylation of the GlcNAc to form GlcN-PI, (ii) the transfer of three mannose residues from dolichol-phosphate-mannose to form Man3GlcN-PI, (iii) the acylation of the inositol ring and transfer of ethanolamine phosphate (EtN-P) to form EtN-P-Man3GlcN-acyl-PI, and (iv) the sequential remodeling of the sn-1 and sn-2 fatty acids (primarily C18:0) with myristate (C14:0). The latter remodeling reactions may be initiated on precursors containing either diacyl-PI or inositol-acylated lyso-PI lipid moieties (128, 222). The final products of this pathway are glycolipid A and glycolipid C (an inositol-acylated form of glycolipid A) (128). Only glycolipid A is added to VSG in vitro and in vivo (197), and the precise function of glycolipid C is still unclear. The inositol acylation of glycolipid A to form glycolipid C is a highly dynamic and reversible process. It has been proposed that glycolipid C could constitute a pool of reserve precursors (128-130), or it may be the first intermediate in a catabolic pathway to remove excess intermediates (216).

FIG. 7.
GPI biosynthetic pathways in T. brucei BF and Leishmania promastigotes. The T. brucei pathway has been reviewed in reference 101 and incorporates data from recent studies (222). The L. mexicana pathway is from references 146 and 278. The protein anchor ...

A similar pathway of GPI biosynthesis occurs in T. brucei procyclics, Leishmania promastigotes, and T. cruzi epimastigotes. The mature GPI anchor precursor in T. brucei procyclics contain an inositol-acylated lyso-PI lipid moiety (107). As this end product is identical to the first intermediate in the T. brucei BF fatty acid remodeling pathway (222), it is likely that the procyclic stage lacks one or more enzymes or cofactors involved in transferring myristol groups to the sn-2 position. In Leishmania spp., the protein anchor precursors are assembled on a very minor pool of alkylacyl-PI rather than diacyl-PI molecular species. Interestingly, the sn-2 fatty acid in the Leishmania GPI protein anchor precursors is also exchanged for myristate, although the mature precursors retain a very long (C24:0 or C26:0) alkyl chain at the sn-1 position and are therefore more hydrophobic than the VSG anchor (278). A proportion of the Leishmania protein anchor pool is also inositol acylated. The addition of this modification appears to be highly regulated, as it does not occur on the far more abundant and structurally related free GPIs in the same cell (146). The protein anchor precursors are also assembled on alkylacyl-PI in T. cruzi (3, 141). GPI proteins in the epimastigote stage retain an alkylacyl-PI, while GPI proteins in the infective metacyclic stages can contain either alkylacyl-PI (on IG7, gp90) or inositolphosphoceramide (3, 6, 140). The presence of these protein-specific anchor lipids could reflect the presence of different GPI precursors. Alternatively, all proteins may receive the same anchor and then be subjected to protein-specific alkylacylglycerol:ceramide remodeling reactions, analogous to those identified in yeast (34, 284) (Fig. (Fig.6B).6B). Interestingly, differences in the lipid moiety may define the rate of turnover of surface-expressed proteins. Proteins containing a ceramide moiety are shed from the surface of T. cruzi as membrane blebs, while those containing alkylacylglycerol are apparently excluded from this process (123, 304). The GPI anchors of the mucins in T. cruzi trypomastigotes contain an alkylacyl-PI with unsaturated fatty acids (C18:1 or C18:2) (8). These GPIs are among the most potent stimulators of macrophage proinflammatory cytokines and may be important in inducing some of the pathology seen in Chagasic patients (8). Finally, some T. cruzi GPI protein anchor precursors may be modified with terminal aminoethyl-phosphonate, which forms a novel bridge between the protein and the mature GPI anchor (3, 141) (Fig. (Fig.6B6B).

GPI anchor precursors are rapidly attached to newly synthesized VSG in the ER lumen (23, 97). In yeast and animal cells, this process is catalyzed by a heterodimeric complex of two integral membrane proteins, GPI8p and Gaa1p, which removes the C-terminal signal sequence of the nascent protein and simultaneously attaches the newly exposed C terminus to the ethanolamine of the GPI precursor. GPI8p shares sequence homology with other endopeptidases and is proposed to be the catalytic component. This reaction has recently been reconstituted in vitro by using a trypanosome cell-free system (322) and an in vitro translation system (86). Unexpectedly, the GPI8p activity in trypanosome membranes can be readily extracted in high pH salt buffers, suggesting that it is a soluble protein (321). Consistent with this finding, the L. mexicana GPI8 gene is predicted to encode a hydrophilic protein that lacks a distinct transmembrane domain (146). The leishmanial GPI8p also lacks an obvious ER retention signal and may depend on interactions with other components of the GPI-transamidase complex (i.e., Gaa1p, PIG-S, and PIG-T) for ER retention (245).

Compartmentalization and topology of GPI biosynthesis.

It is now well established that many of the enzymes involved in phospholipid and sterol biosynthesis are compartmentalized within distinct subdomains of the ER (2, 360). In L. mexicana promastigotes, the enzymes involved in GPI biosynthesis appear to be enriched within a light ER subcompartment (159, 226). These membranes are also enriched in enzymes involved in PI and aminophospholipid biosynthesis (226) (Mullin and McConville, unpublished). The compartmentalization of these enzymes may be required to sustain the extraordinarily high levels of GPI biosynthesis in these parasites. However, de novo-synthesized PI is incorporated into free GPIs only after a long lag time in vivo and not at all in vitro, suggesting that the entry of PI into this pathway is highly regulated (Mullin and McConville, unpublished).

Intermediates in GPI biosynthesis are thought to be assembled on both sides of the ER membrane. While the initial steps in GPI biosynthesis (up to the formation of GlcN-PI) occur on the cytoplasmic side of the ER, later steps are catalyzed by luminally oriented enzymes (192, 204, 358). However, early studies by Vidugiriene and Menon indicated that a significant fraction of the newly synthesized mannosylated intermediates in T. brucei BF become oriented on the cytoplasmic leaflet of the ER (359). Similarly, Mensa-Wilmot and colleagues have provided evidence that the protein anchor intermediates in L. major promastigotes are quantitatively hydrolyzed in vivo if the T. brucei GPI-PLC is ectopically expressed in these cells (213, 214). As the GPI-PLC lacks an N-terminal signal sequence and is thought to associate with the cytoplasmic leaflet of intracellular membranes (48), these data supported the notion that some protein anchor intermediates are flipped to the cytoplasmic leaflet of the ER. Surprisingly, the levels of expression of free GPIs and LPG are unchanged in L. major and L. mexicana promastigotes expressing the GPI-PLC, suggesting that intermediates in these pathways have a different topology from the protein anchor intermediates (160, 214). However, recent studies suggest that this is not the case (Ralton et al., submitted) and that the phenotype induced by the ectopic expression of GPI-PLC may be more complex than previously thought. Indeed there is evidence that this lipase may be secreted into the flagellar pocket in T. brucei BF (119). As the GPI-PLC is multiply acylated (14, 256), it may be secreted into the flagellar pocket via the nonclassical pathway outlined above. The selective down-regulation of GPI proteins in Leishmania expressing this enzyme could thus be due to hydrolysis of GPI proteins but not free GPIs and LPG within the secretory-endocytic pathway or in the flagellar pocket. Finally, the fact that endogenous and ectopically expressed GPI-PLC does not hydrolyze free GPIs in T. brucei BF and Leishmania spp., respectively, although it can hydrolyze other PI lipids (243), suggests that this enzyme does not associate with ER (and Golgi) membranes.

Golgi and post-Golgi modifications of protein-linked GPIs.

The GPI anchor of different classes of VSG can be variably modified with 0 to 10 galactose residues during transit to the cell surface. While the first galactose residue may be added in the ER, subsequent αGal residues are probably added in the Golgi apparatus (22, 196) (Fig. (Fig.6A).6A). The anchors of different VSG subclasses are modified with galactose to different extents (none in class III, zero to five residues in class I, and up to eight residues in class II), suggesting that the galactosyltransferases act as spatial probes, filling in the space between the membrane and the VSG coat (101, 380). In support of this notion, a small proportion of the free GPIs in T. brucei BF are modified with galactose residues to the same extent, regardless of VSG subtype (196). In T. congolense BF, the VSG anchor is modified with a novel Galβ1-6GlcNAc side chain that is added to the first core mannose residue (118). In addition, the lipid moieties of the VSG anchors can undergo further rounds of fatty acid remodeling in the Golgi or post-Golgi compartment, in which preexisting myristic acid is replaced with another myristic acid (54). These reactions are biochemically distinct from the ER fatty acid remodeling reactions and presumably constitute a proofreading mechanism (54).

In T. brucei procyclics, the GPI anchors of the procyclins are extensively modified with large (5 to 30 hexoses) heterogeneous glycan side chains (102) (Fig. (Fig.6A).6A). These glycan side chains consist of poly-NAL structures that are linked to the GPI backbone and are capped with sialic acid by the cell surface trans-sialidase (269). The addition of the poly-NAL to procyclic anchors is presumed to occur in the Golgi apparatus and is not protein specific, as similar side chains are added to the anchor of ectopically expressed VSG (257, 380). In contrast, the protein-linked GPIs of T. cruzi and Leishmania do not appear to receive any further modifications in the Golgi apparatus and contain only the single mannose extension (added in the ER) or no modifications, respectively (Fig. (Fig.6B6B and andC).C). The lack of modifications on these anchors is in contrast to the extensive Golgi-specific modifications that are added to the more abundant free GPIs of these parasites.

Notable differences between the T. brucei and mammalian and yeast GPI pathways include (i) the timing of inositol acylation and deacylation, (ii) the presence of additional ethanolamine phosphate residues on the glycan backbone of mammalian and yeast but not trypanosomatid GPIs, and (iii) the myristic acid remodeling of T. brucei and Leishmania anchors (100). Several potential inhibitors that exploit differences in the substrate specificity of the trypanosome and mammalian enzymes have been developed (317, 325, 327, 329). Inhibitors of the fatty acid remodeling reactions also have potent trypanocidal activity (81). Recently, Morita and colleagues showed that T. brucei BF can synthesize a major fraction of myristic acid de novo rather than scavenge fatty acids from the host bloodstream as previously thought and that these de novo-synthesized fatty acids are efficiently incorporated into GPIs (223). The fatty acid synthetase activity is associated with microsomal membranes, utilizes butyryl-coenzyme A (butyryl-CoA) instead of acetyl-CoA as a primer, and is inhibited by the antibiotic thiolactomycin, a highly specific inhibitor of prokaryote (but not animal) type II fatty acid synthetases. If de novo-synthesized fatty acids rather than fatty acids taken up from the media are the major source of myristic acid for GPI biosynthesis, these enzymes may be interesting drug targets (223, 258).

Biosynthesis of Leishmania LPG

The LPGs are the major surface macromolecules of most human-pathogenic Leishmania species, although levels of expression are lower in members of the Leishmania braziliensis complex (229) and not detectable in the lizard parasite Leishmania alderi (273). The Leishmania LPGs contain a highly conserved GPI anchor with the structure Galα1-6Galα1-3Galfβ1-3[Glcα1-PO4-6]Manα1-3Manα1-4GlcN-lyso-alkyl-PI. The lipid moiety has the same very long (C24:0 or C26:0) alkyl chains as the protein anchors (205). This anchor structure is subsequently modified with a long phosphoglycan chain comprising 10 to 40 Galβ1-4Manα1-PO4 repeat units. These repeat units are further elaborated with species- and stage-specific side chains and capped with a mannose-rich oligosaccharide (39, 205) (Fig. (Fig.6C6C and and7).7). Many of the steps in the assembly of the LPG anchor and phosphoglycan chain have been studied in vivo and in vitro (58, 59, 278), and a number of genes encoding putative transferases and nucleotide transporters have been identified by complementation of LPG mutants (35; D. E. Dobson, L. D. Scholtes, E. V. Kelli, B. J. Mengeling, D. Sullivan, D. L. Sacks, S. J. Turco, and S. M. Beverley, Mol. Parasitol. Meet. XI, abstr. 101, 2000). The LPG anchors are assembled on the same minor pool of alkylacyl-PI as the protein anchor precursors (278) (Fig. (Fig.7).7). However, this pathway diverges from the protein anchor pathway with the addition of the second mannose residue in α1-3 rather than α1-6 linkage. The α1-3-linked mannose is probably added on the cytoplasmic face of the ER by a GDP-Man-dependent mannosyltransferase (160, 280). In contrast, all the other GPI mannosylation reactions are thought to occur in the ER lumen (204). The LPG anchor precursor is subsequently elongated with a galactofuranose residue involving the product of the LPG1 gene (149) (Fig. (Fig.7).7). LPG1p is a type 2 integral membrane protein that is primarily oriented in the lumen of the Golgi apparatus (131). Thus, early LPG intermediates must be flipped from the cytosolic face of the ER to the luminal face of the ER or the Golgi for this step to occur. The remaining steps in LPG anchor synthesis include the addition of two more Gal residues and a Glc-PO4 side chain and deacylation of the lipid moiety (Fig. (Fig.7).7). However, the ordering and enzymology of these reactions have not been carried out. The phosphoglycan moiety of LPG is subsequently assembled by the multiple rounds of Man-1-PO4 and Gal (donated from GDP-Man and UDP-Gal, respectively) additions to the mature anchor and growing chain (58, 59). Mutants lacking the Golgi GDP-Man transporter (the product of the LPG2 gene) are unable to synthesis these phosphoglycan chains, supporting the notion that GDP-Man is the donor for all the mannose additions and that phosphoglycan synthesis occurs in the Golgi apparatus (147, 191). At least two mannose-1-phosphate transferases are required for the assembly of the first repeat and subsequent repeat units, respectively (75, 291). The elongating transferase acts only on unmodified repeat units, demonstrating that the backbone repeat units must be formed before the side chains are added (291). Several enzymes involved in the addition of the species- and stage-specific side chains have recently been characterized by using in vitro assays (40, 233, 234), and genes have been identified by complementation of mutants (51). In L. major, families of galactosyl- and arabinosyltransferases are required for addition of a unique set of glycan side chains to the LPG phosphoglycan backbone. As L. major procyclic promastigotes differentiate into nondividing metacyclic promastigotes, the average length of the LPG chains increases (~2-fold) and the galactose side chains become extensively capped with arabinose-pyranose (Arap) residues (206, 301). The arabinose units are transferred from GDP-Arap (307), which is synthesized in the cytosol and possibly transported into the Golgi by the LPG2p GDP-Man transporter (147). How the developmentally regulated changes in the average length of the LPG phosphoglycan chains and the degree of Ara capping are regulated during promastigote growth remain intriguing questions.

Biosynthesis of Free GPIs

Free GPIs are the major cellular glycolipids in all trypanosomatids investigated to date. In T. brucei BF, the free GPIs are structurally and functionally indistinguishable from the protein anchor precursors and thus appear to be excess products of this pathway. However, in Leishmania, T. cruzi, and many other trypanosomatids, the free GPIs are structurally distinct from the protein anchors and are clearly metabolic end products (71, 72, 200, 201, 203, 282, 310, 377). The function of the free GPIs remains enigmatic. Recent gene knockout studies suggest that they may be essential for growth of L. mexicana promastigotes under some growth conditions (160) but not others (112-114). Down-regulation of free GPIs in T. cruzi amastigotes by ectopic expression of a GPI-PLC also inhibited growth (115). The free GPIs of Leishmania spp. are classified as type 1, type 2, or hybrid, depending on whether they contain the same glycan backbone structure as the protein anchors, the LPG anchors, or the core structures of both anchors, respectively (201). Most species of Leishmania express hybrid-type free GPIs that are assembled on a distinct pool of PI precursors from those incorporated into the protein and LPG anchor precursors (278, 309) (Fig. (Fig.7).7). The steps involved in the assembly of these glycolipids are the same as those involved in protein anchor biosynthesis except that each of the mannosylated intermediates in this pathway may be modified with an α1-3-linked mannose branch (201, 278). Addition of this residue on the cytoplasmic leaflet of the ER may prevent subsequent addition of the α1-6-linked mannose or further extension of this residue, leading to the accumulation of a family of free GPIs with two to four mannose residues (278, 377). The free GPIs of L. major and L. alderi promastigotes have the same glycan head group as the LPG anchor (199, 273, 276, 328). Recent gene deletion experiments suggest that the regulation of the LPG anchor and free GPI biosynthetic pathways is more complex than previously thought. For example, deletion of the L. major LPG1 gene encoding the putative galactofuranose transferase abolishes galactofuranose addition to the LPG anchor precursors but not the free GPIs (335). L. major may thus contain two galactofuranosyltransferases that differentially recognize intermediates in the LPG anchor and free GPI biosynthetic pathways. The differential expression of these different isoforms could account for the selective down-regulation of LPG anchor but not free GPI biosynthesis in the amastigote stage (16, 200, 308).

Following the assembly of the glycan head group and remodeling of the sn-2 fatty acid (278), the free GPIs are transported to the exoplasmic leaflet of the plasma membrane. In L. mexicana, the free GPIs reach the plasma membrane more slowly than the GPI protein gp63 (t1/2, 70 min compared to 40 min) but appear to be transported by the same (temperature-sensitive) vesicular pathway (280). The distinct transport kinetics of these molecules could reflect the facilitated transport of gp63 out of the ER (see above) while the free GPIs are transported by bulk flow. Upon reaching the plasma membrane, the hybrid free GPIs of L. mexicana are incorporated into detergent-resistant domains in the exoplasmic leaflet of the plasma membrane and may themselves be important constituents in maintaining these domains (280).

Protein O Glycosylation

Trypanosomatids do not appear to modify any of the proteins in the secretory pathway with O-linked GalNAc or mannose residues, the major types of O-linked glycans in vertebrate cells and fungi, respectively. In contrast, several mucin-like glycoproteins on the surfaces of T. cruzi epimastigotes, metacyclic trypomastigotes, and amastigotes are extensively modified with O-linked αGlcNAc residues that are added to Thr-rich sequences in these proteins (3, 9, 117, 272, 274, 304) (Fig. (Fig.6).6). This type of modification is unique among the trypanosomatids and is different from addition of O-βGlcNAc to intracellular proteins (134). Most of the O-GlcNAc on the T. cruzi mucins is extended with one to five galactose residues that form short linear and branched glycan chains (3, 9, 274, 348) (Fig. (Fig.6B).6B). Terminal β-Gal residues in these glycans are the major acceptors for the cell surface trans-sialidases that transfer sialic acid (one or two residues per chain) from host glycoconjugates (304). The structures of these O-linked glycans can exhibit some strain-specific polymorphisms. In particular, in the T. cruzi Y strain, all the O-linked galactose residues are in the pyranose configuration, while in the G strain some of these residues are in the furanose configuration (9). Moreover, some of the O-glycans on the high-molecular-weight mucins of the mammalian stages are modified with O-glycans that terminate in Galα1-3Galβ1-4GlcNAc (9). These αGal epitopes are highly immunogenic to humans and are recognized by lytic antibodies in the sera of patients with acute and chronic Chagas' disease (9).

The GlcNAc-transferase that initiates O glycosylation in T. cruzi is associated with purified Golgi membranes, utilizes UDP-GlcNAc as the sugar donor, and adds GlcNAc residues to Thr residues in a synthetic dodecapeptide containing the consensus sequence of the T. cruzi MUC gene (220, 275). The O glycosylation of the T. cruzi mucins is clearly important in forming a protective surface glycocalyx (77). Addition of O-linked glycans may confer structural rigidity to the mucin polypeptide, ensuring that the hypervariable N-terminal domain is presented on the surface of the mucin coat, which may direct the immune response away from conserved domains within the coat (268). As mentioned above, the sialylation of the mucin O-glycans is also important for parasite invasion and protecting the extracellular forms from lysis by complement and the parasite's own hemolysin (261).

Protein Phosphoglycosylation

A number of cell surface and secreted trypanosomatid proteins are elaborated with a distinct class of phosphooligosaccharides. Phosphoglycosylation is initiated by transfer of a sugar-phosphate to Ser or Thr residues in the context of serine/threonine-rich sequences (157, 369). Protein phosphoglycosylation probably occurs in all trypanosomatids and is the most abundant form of protein glycosylation in Leishmania spp. (153). Protein phosphoglycosylation has not been identified in any metazoan organisms to date, although there is increasing evidence that this type of modification (often involving different sugar-phosphate linkages) may be common in other unicellular eukaryotes, such as Dictyostelium discoideum and the protozoan parasite Entamoeba histolytica (137, 219).

This unusual type of glycan modification was initially detected on the abundant secreted acid phosphatase (SAP) of L. donovani and L. mexicana. Early immunochemical and biochemical analyses indicated that these heavily glycosylated proteins were modified with similar phosphoglycans to those found on the LPG of the same parasites (28, 162). Subsequent studies showed that serine residues in the protein backbone of the SAP were modified with Man-1-PO4, which was extended with short linear chains of α1-2-linked mannose or longer chains of repeating Galβ1-4Manα1-PO4-phosphodisaccharides (157, 185, 224). The SAPs belong to a heterogeneous family of PPGs, which include the promastigote filamentous PPG, the GPI-anchored cell surface PPG, and the nonfilamentous amastigote PPG (153, 155, 156). The distinct polypeptide backbones of these PPGs contain Ser/Thr-rich or Ser/Pro-rich domains that are extensively modified with phosphoglycan chains (156, 369). The length and composition of the phosphoglycan chains vary enormously in different PPGs (157, 158). While the 100-kDa form of L. mexicana SAP is primarily modified with short (one to six residues long) mannose oligosaccharides, the secreted PPGs of the amastigote stage are elaborated with exceedingly complex branched phosphoglycans (154). The assembly of phosphoglycan chains may thus depend on the properties of the protein carrier, the rate at which these proteins are transported through the secretory pathway, as well as the complement of glycosyltransferases expressed in each species (368). While some of the SAPs of Old World Leishmania spp. are monomeric, the SAPs of New World species (L. mexicana, Leishmania amazonensis, and L. braziliensis) assemble into highly unusual polymeric chains, containing up to 200 subunits (~2 μm long) (342). These chains are not present in the Golgi but appear to assemble in the flagellar pocket (341). As the filamentous PPGs (encoded by a 23-kb gene and containing 96% carbohydrate) are as long as ~2 μm (153), it is highly likely that the majority of these molecules are retained with the lumen of the Golgi cisternae and transported across the Golgi stack by cisternal maturation. Similarly, transport from the TGN to the plasma membrane may be in large cisternal vacuoles (226, 365).

In T. cruzi, the stage-specific glycoprotein gp72 is heavily phosphoglycosylated (Fig. (Fig.6B).6B). This glycoprotein is required for attachment of the flagellum to the cell body of epimastigotes and metacyclic stages (64). Approximately 50% of the mass of the protein comprises complex glycans (containing xylose, rhamnose, fucose, and galactofuranose residues) that are recognized by the antibody WIC 29.26 (138). These glycans are released by mild acid hydrolysis and are probably linked to phosphothreonine and some phosphoserine residues in the polypeptide backbone (138). Recent studies by Haynes et al. and Ferguson and colleagues suggest that these glycans have the partial structure Galfβ1-4Rhaα1-2Fucα1-2/3[PO4-5/6Galfβ1-2/3]Galfβ1-4Xylβ1-4Xyl-PO4-Thr/Ser (138; M. Ferguson, personal communication). Interestingly, T. brucei BF and procyclics express a homologue of GP72 (Fla1) that also associates with the flagellar attachment zone and is modified with both N-glycans and (in the case of BF) acid-labile oligosaccharides (241). To date, there is no information on either the function or the site of synthesis of these novel oligosaccharides.


Considerable progress has been made in the last few years in defining the ultrastructure of the secretory and endocytic pathways of the trypanosomatids and the nature of protein and lipid transport routes within these pathways. These studies have been greatly facilitated by the identification of organelle-specific markers and cargo proteins, the characterization of the biosynthetic functions of the ER and Golgi apparatus, and, more recently, the identification of genes (via genome searches) that regulate organelle biogenesis and intraorganelle transport. Collectively, these studies demonstrate that the basic features of the trypanosomatid secretory-endocytic pathways are very similar to those found in other eukaryotes, despite the fact that these organisms represent one of the most divergent eukaryotic lineages. In this respect, the trypanosomatids may prove to be interesting experimental systems for investigating aspects of protein and lipid trafficking and glycan and lipid biosynthesis that are highly up-regulated and may have been conserved throughout eukaryotic evolution, such as the transport of GPI proteins. These studies are facilitated by the fact that all the major organelles in the secretory and endocytic pathways can be readily visualized at the level of light and electron microscopy. On the other hand, some aspects of the trypanosomatid secretory and endocytic pathways are clearly unusual. It remains to be determined how the highly polarized secretory and endocytic pathways of these parasites are maintained in the presence of a minimalist system of cytoplasmic microtubules and the nature of sorting signals that direct proteins to the unusual acidocalcisomes. The recent discovery of the exotic lysosome-MVT of Leishmania promastigotes and the related late-endosome-MVT of T. cruzi epimastigotes highlights the importance of visualizing these structures in live cells and the need to undertake comparative studies of all developmental stages. With the sequencing of the genomes of T. brucei, L. major, and T. cruzi well advanced, the stage is now set to increase our understanding of the molecular basis underlying protein and lipid transport and organelle biogenesis in these important parasites. This information may in turn lead to the development of new antiparasite strategies.


We thank Jay Bangs, Mark Field, Mike Ferguson, and Dee Sharma for communicating unpublished data, Ross Waller, Yasu Morita, and Julie Ralton for critical reading of the manuscript, and other members of the McConville laboratory for comments and suggestions.

Work from our laboratory cited in this article was funded by the Australian National Health and Medical Research Council, the Australian Research Council, and the Wellcome Trust. M.J.M. is a Howard Hughes International Scholar.


1. Ace, T. A., S. Gokool, D. McGhie, S. Stager, and D. F. Smith. 1999. Expression of hydrophilic surface proteins in infective stages of Leishmania donovani. Mol. Biochem. Parasitol. 102:191-196. [PubMed]
2. Achleitner, G., B. Gaigg, A. Krasser, E. Kainersdorfer, S. D. Kohlwein, A. Perktold, G. Zellnig, and G. Daum. 1999. Association between the endoplasmic reticulum and mitochondria of yeast facilitates interorganelle transport of phospholipids through membrane contacts. Eur. J. Biochem. 264:545-553. [PubMed]
3. Acosta Serrano, A., S. Schenkman, N. Yoshida, A. Mehlert, J. M. Richardson, and M. A. J. Ferguson. 1995. The lipid structure of the glycosylphosphatidylinositol-anchored mucin-like sialic acid acceptors of Trypanosoma cruzi changes during parasite differentiation from epimastigotes to infective metacyclic trypomastigote forms. J. Biol. Chem. 270:27244-27253. [PubMed]
4. Acosta-Serrano, A., I. C. Almeida, L. H. Freitas-Junior, N. Yoshida, and S. Schenkman. 2001. The mucin-like glycoprotein super-family of Trypanosoma cruzi: structure and biological roles. Mol. Biochem. Parasitol. 114:143-150. [PubMed]
5. Acosta-Serrano, A., R. N. Cole, and P. T. Englund. 2000. Killing of Trypanosoma brucei by concanavalin A: structural basis of resistance in glycosylation mutants. J. Mol. Biol. 304:633-644. [PubMed]
6. Agusti, R., A. S. Couto, O. E. Campetella, A. C. Frasch, and R. M. de Lederkremer. 1997. The trans-sialidase of Trypanosoma cruzi is anchored by two different lipids. Glycobiology 7:731-735. [PubMed]
7. Reference deleted.
8. Almeida, I. C., M. M. Camargo, D. O. Procopio, L. S. Silva, A. Mehlert, L. R. Travassos, R. T. Gazzinelli, and M. A. Ferguson. 2000. Highly purified glycosylphosphatidylinositols from Trypanosoma cruzi are potent proinflammatory agents. EMBO J. 19:1476-1485. [PubMed]
9. Almeida, I. C., M. A. J. Ferguson, S. Schenkman, and L. R. Travassos. 1994. Lytic anti-α-galactosyl antibodies from patients with chronic Chagas' disease recognize novel O-linked oligosaccharides on mucin-like glycosyl-phosphatidylinositol-anchored glycoproteins of Trypanosoma cruzi. Biochem. J. 304:793-802. [PubMed]
10. Al-Qahtani, A., M. Teilhet, and K. Mensa-Wilmot. 1998. Species-specificity in endoplasmic reticulum signal peptide utilization revealed by proteins from Trypanosoma brucei and Leishmania. Biochem. J. 331:521-529. [PubMed]
11. Andrei, C., C. Dazzi, L. Lotti, M. R. Torrisi, G. Chimini, and A. Rubartelli. 1999. The secretory route of the leaderless protein interleukin 1β involves exocytosis of endolysosome-related vesicles. Mol. Biol. Cell 10:1463-1475. [PMC free article] [PubMed]
12. Andrews, N. W. 2000. Regulated secretion of conventional lysosomes. Trends Cell Biol. 10:316-321. [PubMed]
13. Andrews, N. W., C. K. Abrams, S. L. Slatin, and G. Griffiths. 1990. A T. cruzi-secreted protein immunologically related to the complement component C9: evidence for membrane pore-forming activity at low pH. Cell 61:1277-1287. [PubMed]
14. Armah, D. A., and K. Mensa-Wilmot. 1999. S-myristoylation of a glycosylphosphatidylinositol-specific phospholipase C in Trypanosoma brucei. J. Biol. Chem. 274:5931-5938. [PubMed]
15. Bagnat, M., S. Keranen, A. Shevchenko, and K. Simons. 2000. Lipid rafts function in biosynthetic delivery of proteins to the cell surface in yeast. Proc. Natl. Acad. Sci. USA 97:3254-3259. [PubMed]
16. Bahr, V., Y. D. Stierhof, T. Ilg, M. Demar, M. Quinten, and P. Overath. 1993. Expression of lipophosphoglycan, high-molecular weight phosphoglycan and glycoprotein 63 in promastigotes and amastigotes of Leishmania mexicana. Mol. Biochem. Parasitol. 58:107-121. [PubMed]
17. Bakalara, N., X. Santarelli, C. Davis, and T. Baltz. 2000. Purification, cloning, and characterization of an acidic ectoprotein phosphatase differentially expressed in the infectious bloodstream form of Trypanosoma brucei. J. Biol. Chem. 275:8863-8871. [PubMed]
18. Balber, A. E., J. D. Bangs, S. M. Jones, and R. L. Proia. 1979. Inactivation or elimination of potentially trypanolytic complement-activating immune complexes by pathogenic trypanosomes. Infect. Immun. 24:617-627. [PMC free article] [PubMed]
19. Bangs, J. D. 1998. Surface coats and secretory trafficking in African trypanosomes. Curr. Opin. Microbiol. 1:448-454. [PubMed]
20. Bangs, J. D., N. W. Andrews, G. W. Hart, and P. T. Englund. 1986. Posttranslational modification and intracellular transport of a trypanosome variant surface glycoprotein. J. Cell Biol. 103:255-263. [PMC free article] [PubMed]
21. Bangs, J. D., E. M. Brouch, D. M. Ransom, and J. L. Roggy. 1996. A soluble secretory reporter system in Trypanosoma brucei—studies on endoplasmic reticulum targeting. J. Biol. Chem. 271:18387-18393. [PubMed]
22. Bangs, J. D., T. L. Doering, P. T. Englund, and G. W. Hart. 1988. Biosynthesis of a variant surface glycoprotein of Trypanosoma brucei. Processing of the glycolipid membrane anchor and N-linked oligosaccharides. J. Biol. Chem. 263:17697-17705. [PubMed]
23. Bangs, J. D., D. Hereld, J. L. Krakow, G. W. Hart, and P. T. Englund. 1985. Rapid processing of the carboxyl terminus of a trypanosome variant surface glycoprotein. Proc. Natl. Acad. Sci. USA 82:3207-3211. [PubMed]
24. Bangs, J. D., D. M. Ransom, M. A. McDowell, and E. M. Brouch. 1997. Expression of bloodstream variant surface glycoproteins in procyclic stage Trypanosoma brucei—role of GPI anchors in secretion. EMBO J. 16:4285-4294. [PubMed]
25. Bangs, J. D., L. Uyetake, M. J. Brickman, A. E. Balber, and J. C. Boothroyd. 1993. Molecular cloning and cellular localization of a Bip homologue in Trypanosoma brucei; divergent ER retention signals in a lower eukaryote. J. Cell Sci. 105:1101-1113. [PubMed]
26. Barret, M. P., E. Tetaud, A. Seyfang, F. Bringaud, and T. Baltz. 1998. Trypanosome glucose transporters. Mol. Biochem. Parasitol. 91:195-205. [PubMed]
27. Bastin, P., A. Stephan, J. Raper, J. M. Saint-Remy, F. R. Opperdoes, and P. J. Coutoy. 1996. An Mr 145,000 low-density lipoprotein (LDL)-binding protein is conserved throughout the Kinetoplastida order. Mol. Biochem. Parasitol. 76:43-56. [PubMed]
28. Bates, P. A., I. Hermes, and D. M. Dwyer. 1990. Golgi-mediated post-translational processing of secretory acid phosphatase by Leishmania donovani promastigotes. Mol. Biochem. Parasitol. 39:247-255. [PubMed]
29. Becker, B., and M. Melkonian. 1996. The secretory pathway of protists: spatial and functional organization and evolution. Microbiol. Rev. 60:697-721. [PMC free article] [PubMed]
30. Benaim, G., C. Lopez-Estrano, R. Docampo, and S. N. J. Moreno. 1993. A calmodulin-stimulated Ca2+ pump in plasma-membrane vesicles from Trypanosoma brucei; selective inhibition by pentamidine. Biochem. J. 296:759-763. [PubMed]
31. Benchimol, M., W. De Souza, N. Vanderheyden, L. Zhong, H. G. Lu, S. N. Moreno, and R. Docampo. 1998. Functional expression of a vacuolar-type H+-ATPase in the plasma membrane and intracellular vacuoles of Trypanosoma cruzi. Biochem. J. 332:695-702. [PubMed]
32. Benchimol, M., K. C. Ribeiro, R. M. Mariante, and J. F. Alderete. 2001. Structure and division of the Golgi complex in Trichomonas vaginalis and Tritrichomonas foetus. Eur. J. Cell Biol. 80:593-607. [PubMed]
33. Berberof, M., D. Perez-Morga, and E. Pays. 2001. A receptor-like flagellar pocket glycoprotein specific to Trypanosoma brucei gambiense. Mol. Biochem. Parasitol. 113:127-138. [PubMed]
34. Bertello, L. E., M. J. Alves, W. Colli, and R. M. de Lederkremer. 2000. Evidence for phospholipases from Trypanosoma cruzi active on phosphatidylinositol and inositolphosphoceramide. Biochem. J. 345:77-84. [PubMed]
35. Beverley, S. M., and S. J. Turco. 1998. Lipophosphoglycan (LPG) and the identification of virulence genes in the protozoan parasite Leishmania. Trends Microbiol. 6:35-40. [PubMed]
36. Bloom, G. S., and L. S. B. Goldstein. 1998. Cruising along microtubule highways: how membranes move through the secretory pathway. J. Cell Biol. 140:1277-1280. [PMC free article] [PubMed]
37. Reference deleted.
38. Borst, P., and A. H. Fairlamb. 1998. Surface receptors and transporters of Trypanosoma brucei. Annu. Rev. Microbiol. 52:745-778. [PubMed]
39. Bray, A., D. L. Sacks, E. Saraiva, G. Modi, and S. J. Turco. 1999. Intra- and stage-specific polymorphisms in lipophosphoglycan structure control Leishmania donovani-sandfly interactions. Biochemistry 38:9813-9823. [PubMed]
40. Bray, A., and S. J. Turco. 1999. Characterization of the glucosyltransferases that assemble the side chains of the Indian Leishmania donovani lipophosphoglycan. Arch. Biochem. Biophys. 372:367-374. [PubMed]
41. Brickman, M. J., and A. E. Balber. 1994. Transport of a lysosomal membrane glycoprotein from the Golgi to endosomes and lysosomes via the cell surface in African trypanosomes. J. Cell Sci. 107:3191-200. [PubMed]
42. Brickman, M. J., and A. E. Balber. 1990. Trypanosoma brucei rhodesiense bloodstream forms: surface ricin-binding glycoproteins are localized exclusively in the flagellar pocket and the flagellar adhesion zone. J. Protozool. 37:219-224. [PubMed]
43. Brickman, M. J., J. M. Cook, and A. E. Balber. 1995. Low temperature reversibly inhibits transport from tubular endosomes to a perinuclear, acidic compartment in African trypanosomes. J. Cell Sci. 108:3611-3621. [PubMed]
44. Brooker, B. E. 1971. The fine structure of Crithidia fasciculata with special reference to the organelles involved in the ingestion and digestion of protein. Z. Zellforsch. 116:532-563. [PubMed]
45. Brooks, D. R., L. Tetley, G. H. Coombs, and J. C. Mottram. 2000. Processing and trafficking of cysteine proteases in Leishmania mexicana. J. Cell Sci. 113:4035-4041. [PubMed]
46. Brown, D. A., and E. London. 1998. Functions of lipid rafts in biological membranes. Annu. Rev. Cell Dev. Biol. 14:111-136. [PubMed]
47. Brown, D. A., and E. London. 2000. Structure and function of sphingolipid- and cholesterol-rich membrane rafts. J. Biol. Chem. 275:17221-17224. [PubMed]
48. Bulow, R., G. Griffiths, P. Webster, Y. D. Stierhof, F. R. Opperdoes, and P. Overath. 1989. Intracellular localization of the glycosyl-phosphatidylinositol-specific phospholipase C of Trypanosoma brucei. J. Cell Sci. 93:233-240. [PubMed]
49. Burleigh, B., and N. W. Andrews. 1995. The mechanisms of Trypanosoma cruzi invasion of mammalian cells. Annu. Rev. Microbiol. 49:175-200. [PubMed]
50. Burleigh, B. A., C. W. Wells, M. W. Clarker, and P. R. Gardiner. 1993. An integral membrane glycoprotein associated with an endocytic compartment of Trypanosoma vivax: identification and partial purification. J. Cell Biol. 120:339-352. [PMC free article] [PubMed]
51. Butcher, B. A., S. J. Turco, B. A. Hilty, P. F. Pimenta, M. Panunzio, and D. L. Sacks. 1996. Deficiency in β1,3-galactosyltransferase of a Leishmania major lipophosphoglycan mutant adversely influences the Leishmania-sand fly interaction. J. Biol. Chem. 271:20573-20579. [PubMed]
52. Butikofer, P., T. Malherbe, M. Boschung, and I. Roditi. 2001. GPI-anchored proteins: now you see 'em, now you don't. FASEB J. 15:545-548. [PubMed]
53. Butikofer, P., E. Vassella, S. Ruepp, M. Boschung, G. Civenni, T. Seebeck, A. Hemphill, N. Mookherjee, T. W. Pearson, and I. Roditi. 1999. Phosphorylation of a major GPI-anchored surface protein of Trypanosoma brucei during transport to the plasma membrane. J. Cell Sci. 112:1785-1795. [PubMed]
54. Buxbaum, L. U., J. Raper, F. R. Opperdoes, and P. T. Englund. 1994. Myristate exchange. A second glycosyl phosphatidylinositol myristoylation reaction in African trypanosomes. J. Biol. Chem. 269:30212-30220. [PubMed]
55. Caffrey, C. R., E. Hansell, K. D. Lucas, L. S. Brinen, A. Alvarez Hernandez, J. Cheng, S. L. Gwaltney, W. R. Roush, Y. D. Stierhof, M. Bogyo, D. Steverding, and J. H. McKerrow. 2001. Active site mapping, biochemical properties and subcellular localization of rhodesain, the major cysteine protease of Trypanosoma brucei rhodesiense. Mol. Biochem. Parasitol. 118:61-73. [PubMed]
56. Cappai, R., A. H. Osborn, P. A. Gleeson, and E. Handman. 1993. Cloning and characterization of a Golgi-associated GTP-binding protein homologue from Leishmania major. Mol. Biochem. Parasitol. 62:73-82. [PubMed]
57. Carruthers, V. B., M. Navarro, and G. A. M. Cross. 1996. Targeted disruption of expression site-associated gene-1 in bloodstream form Trypanosoma brucei. Mol. Biochem. Parasitol. 81:65-79. [PubMed]
58. Carver, M. A., and S. J. Turco. 1992. Biosynthesis of lipophosphoglycan from Leishmania donovani: characterization of mannosylphosphate transfer in vitro. Arch. Biochem. Biophys. 295:309-317. [PubMed]
59. Carver, M. A., and S. J. Turco. 1991. Cell-free biosynthesis of lipophosphoglycan from Leishmania donovani. Characterization of microsomal galactosyltransferase and mannosyltransferase activities. J. Biol. Chem. 266:10974-10981. [PubMed]
60. Chen, D. Q., H. Lu, and K. P. Chang. 1999. Replacement of Leishmania N-acetylglucosamine-1-phosphate transferase gene requires episomal rescue. Mol. Biochem. Parasitol. 100:223-227. [PubMed]
61. Clayton, C., T. Hausler, and J. Blattner. 1995. Protein trafficking in kinetoplastid protozoa. Microbiol. Rev. 59:325-344. [PMC free article] [PubMed]
62. Conibear, E., and T. H. Stevens. 1998. Multiple sorting pathways between the late Golgi and the vacuole in yeast. Biochim. Biophys. Acta 1404:211-230. [PubMed]
63. Coombs, G. H., L. Tetley, V. A. Moss, and K. Vickerman. 1986. Three-dimensional structure of the Leishmania amastigote as revealed by computer-aided reconstruction from serial section. Parasitology 92:13-23. [PubMed]
64. Cooper, R., A. R. de Jesus, and G. A. Cross. 1993. Deletion of an immunodominant Trypanosoma cruzi surface glycoprotein disrupts flagellum-cell adhesion J. Cell Biol. 122:149-156. [PMC free article] [PubMed]
65. Coppens, I., F. R. Opperdoes, P. J. Courtoy, and P. Baudhuin. 1987. Receptor-mediated endocytosis in the bloodstream form of Trypanosoma brucei. J. Protozool. 34:465-473. [PubMed]
66. Couto, A. S., M. F. Goncalves, W. Colli, and R. M. de Lederkremer. 1990. The N-linked carbohydrate chain of the 85-kilodalton glycoprotein from Trypanosoma cruzi trypomastigotes contains sialyl, fucosyl and galactosyl (α1-3)galactose units. Mol. Biochem. Parasitol. 39:101-107. [PubMed]
67. Cross, G. A., and G. B. Takle. 1993. The surface trans-sialidase family of Trypanosoma cruzi. Annu. Rev. Microbiol. 47:385-411. [PubMed]
68. Debrabant, A., E. Ghedin, and D. M. Dwyer. 2000. Dissection of the functional domains of the Leishmania surface membrane 3′-nucleotidase/nuclease, a unique member of the class I nuclease family. J. Biol. Chem. 275:16366-16372. [PubMed]
69. Debrabant, A., M. Gottlieb, and D. M. Dwyer. 1995. Isolation and characterization of the gene encoding the surface membrane 3′-nucleotidase/nuclease of Leishmania donovani. Mol. Biochem. Parasitol. 71:51-63. [PubMed]
70. de Lederkremer, R. M., and W. Colli. 1995. Galactofuranose-containing glycoconjugates in trypanosomatids. Glycobiology 5:547-552. [PubMed]
71. de Lederkremer, R. M., C. Lima, M. I. Ramirez, M. A. Ferguson, S. W. Homans, and J. Thomas-Oates. 1991. Complete structure of the glycan of lipopeptidophosphoglycan from Trypanosoma cruzi epimastigotes. J. Biol. Chem. 266:23670-23675. [PubMed]
72. de Lederkremer, R. M., C. E. Lima, M. I. Ramirez, M. F. Goncalvez, and W. Colli. 1993. Hexadecylpalmitoylglycerol or ceramide is linked to similar glycophosphoinositol anchor-like structures in Trypanosoma cruzi. Eur. J. Biochem. 218:929-936. [PubMed]
73. Denny, P. W., M. C. Field, and D. F. Smith. 2001. GPI-anchored proteins and glycoconjugates segregate into lipid rafts in Kinetoplastida. FEBS Lett. 491:148-153. [PubMed]
74. Denny, P. W., S. Gokool, D. G. Russell, M. C. Field, and D. F. Smith. 2000. Acylation-dependent protein export in Leishmania. J. Biol. Chem. 275:11017-11025. [PubMed]
75. Descoteaux, A., B. J. Mengeling, S. M. Beverley, and S. J. Turco. 1998. Leishmania donovani has distinct mannosylphosphoryltransferases for the initiation and elongation phases of lipophosphoglycan repeating unit biosynthesis. Mol. Biochem. Parasitol. 94:27-40. [PubMed]
76. Descoteaux, A., and S. J. Turco. 1999. Glycoconjugates in Leishmania infectivity. Biochim. Biophys. Acta 1455:341-352. [PubMed]
77. Di Noia, J. M., G. D. Pollevick, M. T. Xavier, J. O. Previato, L. Mendoca-Previato, D. O. Sanchez, and A. C. Frasch. 1996. High diversity in mucin genes and mucin molecules in Trypanosoma cruzi. J. Biol. Chem. 271:32078-32083. [PubMed]
78. Reference deleted.
79. Docampo, R., and S. N. J. Moreno. 2001. The acidocalcisome. Mol. Biochem. Parasitol. 33:151-159. [PubMed]
80. Docampo, R., and S. N. J. Moreno. 1999. Acidocalcisomes: a novel Ca2+ storage compartment in trypanosmatids and apicomplexan parasites. Parasitol. Today 15:443-448. [PubMed]
81. Doering, T. L., J. Raper, L. U. Buxbaum, S. P. Adams, J. I. Gordon, G. W. Hart, and P. T. Englund. 1991. An analog of myristic acid with selective toxicity for African trypanosomes. Science 252:1851-1854. [PubMed]
82. Doering, T. L., and R. Schekman. 1996. GPI anchor attachment is required for Gas1p transport from the endoplasmic retirulum in COP II vesicles. EMBO J. 15:182-191. [PubMed]
83. Drew, M. E., C. K. Langford, E. M. Klamo, D. G. Russell, M. P. Kavanaugh, and S. M. Landfear. 1995. Functional expression of a myo-inositol/H+ symporter from Leishmania donovani. Mol. Cell. Biol. 15:5508-5515. [PMC free article] [PubMed]
84. Duboise, S. M., M. A. Vannier-Santos, D. Costa-Pinto, L. Rivas, A. A. Pan, Y. Traub-Cseko, W. De Souza, and D. McMahon-Pratt. 1994. The biosynthesis, processing, and immunolocalization of Leishmania pifanoi amastigote cysteine proteinases. Mol. Biochem. Parasitol. 68:119-132. [PubMed]
85. Duszenko, M., I. E. Ivanov, M. A. Ferguson, H. Plesken, and G. A. Cross. 1988. Intracellular transport of a variant surface glycoprotein in Trypanosoma brucei. J. Cell Biol. 106:77-86. [PMC free article] [PubMed]
86. Duszenko, M., X. Kang, U. Bohme, R. Homke, and M. Lehner. 1999. In vitro translation in a cell-free system from Trypanosoma brucei yields glycosylated and glycosylphosphatidylinositol-anchored proteins. Eur. J. Biochem. 266:789-797. [PubMed]
87. Dutoya, S., S. Gibert, G. Lemercier, X. Santarelli, D. Baltz, T. Baltz, and N. Bakalara. 2001. A novel C-terminal kinesin is essential for maintaining functional acidocalcisomes in Trypanosoma brucei. J. Biol. Chem. 276:49117-49124. [PubMed]
88. Reference deleted.
89. El-Sayed, N. M., C. M. Alarcon, J. C. Beck, V. C. Sheffield, and J. E. Donelson. 1995. cDNA expressed sequence tags of Trypanosoma brucei rhodesiense provide new insights into the biology of the parasite. Mol. Biochem. Parasitol. 73:75-90. [PubMed]
90. El-Sayed, N. M. A., and J. E. Donelson. 1997. African trypanosomes have differentially expressed genes encoding homologues of the Leishmania GP63 surface protease. J. Biol. Chem. 272:26742-26748. [PubMed]
91. Reference deleted.
92. Engel, J. C., P. S. Doyle, I. Hsieh, and J. H. McKerrow. 1998. Cysteine protease inhibitors cure an experimental Trypanosoma cruzi infection. J. Exp. Med. 188:725-734. [PMC free article] [PubMed]
93. Engel, J. C., P. S. Doyle, J. Palmer, I. Hsieh, D. F. Bainton, and J. H. McKerrow. 1998. Cysteine protease inhibitors alter Golgi complex ultrastructure and function in Trypanosoma cruzi. J. Cell Sci. 111:597-606. [PubMed]
94. Engel, J. C., C. T. Garcia, I. Hsieh, P. S. Doyle, and J. H. McKerrow. 2000. Upregulation of the secretory pathway in cysteine protease inhibitor-resistant Trypanosoma cruzi. J. Cell Sci. 113:1345-1354. [PubMed]
95. Engstler, M., G. Reuter, and R. Schauer. 1993. The developmentally regulated trans-sialidase from Trypanosoma brucei sialylates the procyclic acidic repetitive protein. Mol. Biochem. Parasitol. 61:1-13. [PubMed]
96. Felibertt, P., R. Bermudez, V. Cervino, K. Dawidowicz, F. Dagger, T. Proverbio, R. Marin, and G. Benaim. 1995. Oubain-sensitive Na+, K+-ATPase in the plasma membrane of Leishmania mexicana. Mol. Biochem. Parasitol. 74:179-187. [PubMed]
97. Ferguson, M. A., M. Duszenko, G. S. Lamont, P. Overath, and G. A. Cross. 1986. Biosynthesis of Trypanosoma brucei variant surface glycoproteins. N-glycosylation and addition of a phosphatidylinositol membrane anchor. J. Biol. Chem. 261:356-362. [PubMed]
98. Reference deleted.
99. Ferguson, M. A. J. 2000. Glycosylphosphatidylinositol biosynthesis validated as a drug target for African sleeping sickness. Proc. Natl. Acad. Sci. USA 97:10673-10675. [PubMed]
100. Ferguson, M. A. J. 1999. The structure, biosynthesis and functions of glycosylphosphatidylinositol anchors, and the contributions of trypanosome research. J. Cell Sci. 112:2799-2809. [PubMed]
101. Ferguson, M. A. J., J. S. Brimacombe, J. R. Brown, A. Crossman, A. Dix, R. A. Field, M. L. S. Guther, K. G. Milne, D. K. Sharma, and T. K. Smith. 1999. The GPI biosynthetic pathway as a therapeutic target for African sleeping sickness. Biochim. Biophys. Acta 1455:327-340. [PubMed]
102. Ferguson, M. A. J., P. Murray, H. Rutherford, and M. J. McConville. 1993. A simple purification of procyclic acidic repetitive protein and demonstration of a sialylated glycosyl-phosphatidylinositol membrane anchor. Biochem. J. 291:51-55. [PubMed]
103. Field, H., B. R. S. Ali, T. Sherwin, K. Gull, S. L. Croft, and M. C. Field. 1999. TbRab2p, a marker for the endoplasmic reticulum of Trypanosoma brucei, localises to the ERGIC in mammalian cells. J. Cell Sci. 112:147-156. [PubMed]
104. Field, H., M. Farjah, A. Pal, K. Gull, and M. C. Field. 1998. Complexity of trypanosomatid endocytosis pathways revealed by Rab4 and Rab5 isoforms in Trypanosoma brucei. J. Biol. Chem. 273:32102-32110. [PubMed]
105. Field, H., T. Sherwin, A. C. Smith, K. Gull, and M. C. Field. 2000. Cell-cycle and developmental regulation of TbRAB31 localisation, a GTP-locked Rab protein from Trypanosoma brucei. Mol. Biochem. Parasitol. 106:21-35. [PubMed]
106. Field, M. C., B. R. S. Ali, and H. Field. 1999. GTPases in protozoan parasites: tools for cell biology and chemotherapy. Parasitol. Today 15:365-448. [PubMed]
107. Field, M. C., A. K. Menon, and G. A. Cross. 1991. A glycosylphosphatidylinositol protein anchor from procyclic stage Trypanosoma brucei: lipid structure and biosynthesis. EMBO J. 10:2731-2739. [PubMed]
108. Figueiredo, R. C. B. Q., and M. J. Soares. 1995. The Golgi apparatus of Trypanosoma cruzi epimastigote forms. J. Submicrosc. Cytol. Pathol. 27:209-215. [PubMed]
109. Frasch, A. C. C. 2000. Functional diversity in the trans-sialidase and mucin families in Trypanosoma cruzi. Parasitol. Today 16:282-286. [PubMed]
110. Funk, V. A., A. Jardin, and R. W. Olafson. 1994. An investigation into the significance of N-linked oligosaccharides of Leishmania gp63. Mol. Biochem. Parasitol. 63:23-35. [PubMed]
111. Furuya, T., M. Okura, F. A. Ruiz, D. A. Scott, and R. Docampo. 2001. TcSCA complements yeast mutants defective in Ca2+ pumps and encodes a Ca2+-ATPase that localizes to the endoplasmic reticulum of Trypanosoma cruzi. J. Biol. Chem. 276:32437-32445. [PubMed]
112. Garami, A., and T. Ilg. 2001. Disruption of mannose activation in Leishmania mexicana: GDP-mannose pyrophosphorylase is required for virulence, but not for viability. EMBO J. 20:3657-3666. [PubMed]
113. Garami, A., and T. Ilg. 2001. The role of phosphomannose isomerase in Leishmania mexicana glycoconjugate synthesis and virulence. J. Biol. Chem. 276:6566-6575. [PubMed]
114. Garami, A., A. Mehlert, and T. Ilg. 2001. Glycosylation defects and virulence phenotypes of Leishmania mexicana phosphomannomutase and dolicholphosphate-mannose synthase gene deletion mutants. Mol. Cell. Biol. 21:8168-8183. [PMC free article] [PubMed]
115. Garg, N., M. Postan, K. Mensa-Wilmot, and R. L. Tarleton. 1997. Glycosylphosphatidylinositols are required for the development of Trypanosoma cruzi amastigotes. Infect. Immun. 65:4055-4060. [PMC free article] [PubMed]
116. Garg, N., R. L. Tarleton, and K. Mensa-Wilmot. 1997. Proteins with glycosylphosphatidylinositol (GPI) signal sequences have divergent fates during a GPI deficiency. GPIs are essential for nuclear division in Trypanosoma cruzi. J. Biol. Chem. 272:12482-12491. [PubMed]
117. Gazzinelli, R. T., M. M. Camargo, L. R. Travassos, M. A. J. Ferguson, and I. C. Almeida. 1997. Glycosylphosphatidylinositol anchored mucin-like glycoproteins (GPI-mucins) purified from Trypanosoma cruzi intracellular amastigotes are potent inducers of pro-inflammatory cytokines and nitric oxide by macrophages. Mem. Inst. Oswaldo Cruz 92:135-142. [PubMed]
118. Gerold, P., B. Striepen, B. Reitter, H. Geyer, R. Geyer, E. Reinwald, H. J. Risse, and R. T. Schwarz. 1996. Glycosyl-phosphatidylinositols of Trypanosoma congolense: two common precursors but a new protein-anchor. J. Mol. Biol. 261:181-194. [PubMed]
119. Geuskens, M., E. Pays, and M. L. Cardoso de Almeida. 2000. The lumen of the flagellar pocket of Trypanosoma brucei contains both intact and phospholipase C-cleaved GPI anchored proteins. Mol. Biochem. Parasitol. 108:269-275. [PubMed]
120. Ghedin, E., A. Debrabant, J. C. Engel, and D. M. Dwyer. 2001. Secretory and endocytic pathways converge in a dynamic endosomal system in a primitive protozoan. Traffic 2:175-188. [PubMed]
121. Glick, B. S. 2000. Organization of the Golgi apparatus. Curr. Opin. Cell Biol. 12:450-456. [PubMed]
122. Godsel, L. M., and D. Engman. 1999. Flagellar protein localization mediated by a calcium-myristoyl/palmitoyl switch mechanism. EMBO J. 18:2057-2065. [PubMed]
123. Goncalves, M. F., E. S. Umezawa, A. M. Katzin, W. de Souza, M. J. Alves, B. Zingales, and W. Colli. 1991. Trypanosoma cruzi: shedding of surface antigens as membrane vesicles. Exp. Parasitol. 72:43-53. [PubMed]
124. Grab, D. J., P. Webster, and J. D. Lonsdale-Eccles. 1998. Analysis of trypanosomal endocytic organelles using preparative free-flow electrophoresis. Electrophoresis 19:1162-1170. [PubMed]
125. Grab, D. J., P. Webster, Y. Verjee, and J. Lonsdale-Eccles. 1997. Golgi-associated phosphohydrolases in Trypanosoma brucei brucei. Mol. Biochem. Parasitol. 86:127-132. [PubMed]
126. Gruenberg, J. 2001. The endocytic pathway: a mosaic of domains. Nat. Rev. Mol. Cell Biol. 2:721-730. [PubMed]
127. Gull, K. 1999. The cytoskeleton of trypanosomatid parasites. Annu. Rev. Microbiol. 53:629-655. [PubMed]
128. Guther, M. L. S., and M. A. J. Ferguson. 1995. The role of inositol acylation and inositol deacylation in GPI biosynthesis in Trypanosoma brucei. EMBO J. 14:3080-3093. [PubMed]
129. Guther, M. L. S., W. J. Masterson, and M. A. J. Ferguson. 1994. The effects of phenylmethylsulfonyl fluoride on inositol-acylation and fatty acid remodeling in African trypanosomes. J. Biol. Chem. 269:18694-18701. [PubMed]
130. Guther, M. L. S., W. J. Masterson, and M. A. J. Ferguson. 1994. The role of glycolipid C in the GPI biosynthetic pathway in Trypanosoma brucei bloodstream forms. Braz. J. Med. Biol. Res. 27:121-126. [PubMed]
131. Ha, D. S., J. K. Schwarz, S. J. Turco, and S. M. Beverley. 1996. Use of the green fluorescent protein as a marker in transfected Leishmania. Mol. Biochem. Parasitol. 77:57-64. [PubMed]
132. Hager, K. M., M. A. Pierce, D. R. Moore, E. M. Tyler, J. D. Esko, and S. L. Hajduk. 1994. Endocytosis of a cytotoxic human high density lipoprotein results in disruption of acidic intracellular vesicles and subsequent killing of African trypanosomes. J. Cell Biol. 126:155-167. [PMC free article] [PubMed]
133. Hall, B. F., P. Webster, A. K. Ma, K. A. Joiner, and N. W. Andrews. 1992. Desialylation of lysosomal membrane glycoproteins by Trypanosoma cruzi: a role for the surface neuraminidase in facilitating parasite entry in the host cell cytoplasm. J. Exp. Med. 176:313-325. [PMC free article] [PubMed]
134. Handman, E., L. D. Barnett, A. H. Osborn, J. W. Goding, and P. J. Murray. 1993. Identification, characterization and genomic cloning of an O-linked N-acetylglucosamine-containing cytoplasmic Leishmania glycoprotein. Mol. Biochem. Parasitol. 62:61-72. [PubMed]
135. Handman, E., A. H. Osborn, F. Symons, R. van Driel, and R. Cappai. 1995. The Leishmania promastigote surface antigen 2 complex is differentially expressed during the parasite life cycle. Mol. Biochem. Parasitol. 74:189-200. [PubMed]
136. Harsay, E., and A. Bretscher. 1995. Parallel secretory pathways to the cell surface in yeast. J. Cell Biol. 131:297-310. [PMC free article] [PubMed]
137. Haynes, P. A. 1998. Phosphoglycosylation: a new structural class of glycosylation. Glycobiology 8:1-5. [PubMed]
138. Haynes, P. A., M. A. J. Ferguson, and G. A. M. Cross. 1996. Structural characterization of novel oligosaccharides of cell-surface glycoproteins of Trypanosoma cruzi. Glycobiology 6:869-878. [PubMed]
139. Haynes, P. A., D. G. Russell, and G. A. M. Cross. 1996. Subcellular localization of Trypanosoma cruzi glycoprotein Gp72. J. Cell Sci. 109:2979-2988. [PubMed]
140. Heise, N., M. L. C. Dealmeida, and M. A. J. Ferguson. 1995. Characterization of the lipid moiety of the glycosylphosphatidylinositol anchor of Trypanosoma cruzi 1g7-antigen. Mol. Biochem. Parasitol. 70:71-84. [PubMed]
141. Heise, N., J. Raper, L. U. Buxbaum, T. M. Peranovich, and M. L. de Almeida. 1996. Identification of complete precursors for the glycosylphosphatidylinositol protein anchors of Trypanosoma cruzi. J. Biol. Chem. 271:16877-16887. [PubMed]
142. Hertz-Fowler, C., K. Ersfeld, and K. Gull. 2001. CAP5.5, a life-cycle-regulated, cytoskeleton-associated protein is a member of a novel family of calpain-related proteins in Trypanosoma brucei. Mol. Biochem. Parasitol. 116:25-34. [PubMed]
143. Hill, J. E., D. A. Scott, S. Luo, and R. Docampo. 2000. Cloning and functional expression of a gene encoding a vacuolar-type proton-translocating pyrophosphatase from Trypanosoma cruzi. Biochem. J. 351:281-288. [PubMed]
144. Hill, K. L., N. R. Hutchings, P. M. Grandgenett, and J. E. Donelson. 2000. T lymphocyte-triggering factor of African trypanosomes is associated with the flagellar fraction of the cytoskeleton and represents a new family of proteins that are present in several divergent eukaryotes. J. Biol. Chem. 275:39369-39378. [PubMed]
145. Hill, K. L., N. R. Hutchings, D. G. Russell, and J. E. Donelson. 1999. A novel protein targeting domain directs proteins to the anterior cytoplasmic face of the the flagellar pocket in African trypanosomes. J. Cell Sci. 112:3091-3101. [PubMed]
146. Hilley, J. D., J. L. Zawadzki, M. J. McConville, G. H. Coombs, and J. C. Mottram. 2000. Leishmania mexicana mutants lacking glycosylphosphatidylinositol (GPI):protein transamidase provide insights into the biosynthesis and functions of GPI-anchored proteins. Mol. Biol. Cell 11:1183-1195. [PMC free article] [PubMed]
147. Hong, K., D. Ma, S. M. Beverley, and S. J. Turco. 2000. The Leishmania GDP-mannose transporter is an autonomous, multi-specific, hexameric complex of LPG2 subunits. Biochemistry 39:2013-2022. [PubMed]
148. Horvath, A., C. Sutterlin, U. Manning-Krieg, N. R. Movva, and H. Riezman. 1994. Ceramide synthesis enhances transport of GPI-anchored proteins to the Golgi apparatus in yeast. EMBO J. 13:3687-3695. [PubMed]
149. Huang, C., and S. J. Turco. 1993. Defective galactofuranose addition in lipophosphoglycan biosynthesis in a mutant of Leishmania donovani. J. Biol. Chem. 268:24060-24066. [PubMed]
150. Huete-Perez, J. A., J. C. Engel, L. S. Brinen, J. C. Mottram, and J. H. McKerrow. 1999. Protease trafficking in two primitive eukaryotes is mediated by a prodomain protein motif. J. Biol. Chem. 274:16249-16256. [PubMed]
151. Hwa, K. Y., and K. H. Khoo. 2000. Structural analysis of the asparagine-linked glycans from the procyclic Trypanosoma brucei and its glycosylation mutants resistant to concanavalin A killing. Mol. Biochem. Parasitol. 111:173-184. [PubMed]
152. Ilg, T. 2000. Lipophosphoglycan is not required for infection of macrophages or mice by Leishmania mexicana. EMBO J. 19:1953-1962. [PubMed]
153. Ilg, T. 2000. Proteophosphoglycans of Leishmania. Parasitol. Today 16:489-497. [PubMed]
154. Ilg, T., D. Craik, G. Currie, G. Multhaup, and A. Bacic. 1998. Stage-specific proteophosphoglycan from Leishmania mexicana amastigotes. Structural characterization of novel mono-, di-, and triphosphorylated phosphodiester-linked oligosaccharides. J. Biol. Chem. 273:13509-13523. [PubMed]
155. Ilg, T., E. Handman, and Y.-D. Stierhof. 1999. Proteophosphoglycans from Leishmania promastigotes and amastigotes. Biochem. Soc. Trans. 27:518-525. [PubMed]
156. Ilg, T., J. Montgomery, Y. D. Stierhof, and E. Handman. 1999. Molecular cloning and characterization of a novel repeat-containing Leishmania major gene, ppg1, that encodes a membrane-associated form of proteophosphoglycan with a putative glycosylphosphatidylinositol anchor. J. Biol. Chem. 274:31410-31420. [PubMed]
157. Ilg, T., P. Overath, M. A. J. Ferguson, T. Rutherford, D. G. Campbell, and M. J. McConville. 1994. O- and N-glycosylation of the Leishmania mexicana-secreted acid phosphatase: characterization of a new class of phosphoserine-linked glycans J. Biol. Chem. 269:24073-24081. [PubMed]
158. Ilg, T., Y. D. Stierhof, D. Craik, R. Simpson, E. Handman, and A. Bacic. 1996. Purification and structural characterization of a filamentous, mucin-like proteophosphoglycan secreted by Leishmania parasites. J. Biol. Chem. 271:21583-21596. [PubMed]
159. Ilgoutz, S. C., K. A. Mullin, B. R. Southwell, and M. J. McConville. 1999. Glycosylphosphatidylinositol biosynthetic enzymes are localized to a stable tubular subcompartment of the endoplasmic reticulum in Leishmania mexicana. EMBO J. 18:3643-3654. [PubMed]
160. Ilgoutz, S. C., J. L. Zawadzki, J. E. Ralton, and M. J. McConville. 1999. Evidence that free GPI glycolipids are essential for growth of Leishmania mexicana. EMBO J. 18:2746-2755. [PubMed]
161. Ivens, A. C., S. M. Lewis, A. Bagherzadeh, L. Zhang, H. M. Chan, and D. F. Smith. 1998. A physical map of the Leishmania major Friedlin genome. Genome Res. 8:135-145. [PubMed]
162. Jaffe, C. L., M. L. Perez, and L. F. Schnur. 1990. Lipophosphoglycan and secreted acid phosphatase of Leishmania tropica share species-specific epitopes. Mol. Biochem. Parasitol. 41:233-240. [PubMed]
163. Jeffries, T. R., G. W. Morgan, and M. C. Field. 2001. A developmentally regulated rab11 homologue in Trypanosoma brucei is involved in recycling processes. J. Cell Sci. 114:2617-2626. [PubMed]
164. Joshi, M., G. P. Pogue, R. C. Duncan, N. S. Lee, N. K. Singh, C. D. Atreya, D. M. Dwyer, and H. L. Nakhasi. 1996. Isolation and characterization of Leishmania donovani calreticulin gene and its conservation of the RNA binding activity. Mol. Biochem. Parasitol. 81:53-64. [PubMed]
165. Joshi, P. B., D. L. Sacks, G. Modi, and W. R. McMaster. 1998. Targeted gene deletion of Leishmania major genes encoding developmental stage-specific leishmanolysin (GP63). Mol. Microbiol. 27:519-530. [PubMed]
166. Karp, C. L., S. J. Turco, and D. L. Sacks. 1991. Lipophosphoglycan masks recognition of the Leishmania donovani promastigote surface by human kala-azar serum. J. Immunol. 147:680-684. [PubMed]
167. Kelley, R. J., D. L. Alexander, C. Cowan, A. E. Balber, and J. D. Bangs. 1999. Molecular cloning of p67, a lysosomal membrane glycoprotein from Trypanosoma brucei. Mol. Biochem. Parasitol. 98:17-28. [PubMed]
168. Kelley, R. J., M. J. Brickman, and A. E. Balber. 1995. Processing and transport of a lysosomal membrane glycoprotein is developmentally regulated in African trypanosomes. Mol. Biochem. Parasitol. 74:167-178. [PubMed]
169. Klumperman, J. 2000. Transport between ER and Golgi. Curr. Opin. Cell Biol. 12:445-449. [PubMed]
170. Kundig, C., A. Haimeur, D. Legare, B. Papadopoulou, and M. Ouellette. 1999. Increased transport of pteridines compensates for mutations in the high affinity folate transporter and contributes to methotrexate resistance in the protozoan parasite Leishmania tarentolae. EMBO J. 18:2342-2351. [PubMed]
171. Labriola, C., J. J. Cazzulo, and A. J. Parodi. 1995. Retention of glucose units added by the UDP-Glc:glycoprotein glucosyltransferase delays exit of glycoproteins from the endoplasmic reticulum. J. Cell Biol. 130:771-779. [PMC free article] [PubMed]
172. Labriola, C., J. J. Cazzulo, and A. J. Parodi. 1999. Trypanosoma cruzi calreticulin is a lectin that binds monoglucosylated oligosaccharides but not protein moieties of glycoproteins. Mol. Biol. Cell 10:1381-1394. [PMC free article] [PubMed]
173. Lamb, J. R., V. Fu, E. Wirtz, and J. D. Bangs. 2001. Functional analysis of the trypanosomal AAA protein TbVCP with trans-dominant ATP-hydrolysis mutants. J. Biol. Chem. 276:21512-21520. [PubMed]
174. Landfear, S. M. 2000. Genetics and biochemistry of Leishmania membrane transporters. Curr. Opin. Microbiol. 3:417-421. [PubMed]
175. Landfear, S. M., and M. Ignatushchenko. 2001. The flagellum and flagellar pocket of trypanosomatids. Mol. Biochem. Parasitol. 115:1-17. [PubMed]
176. Langreth, S. G., and A. E. Balber. 1975. Protein uptake and digestion in bloodstream and culture forms of Trypanosoma brucei. J. Protozool. 22:40-53. [PubMed]
177. Leal, S. T., J. R. Araripe, T. P. Urmenyi, G. A. Cross, and E. Rondinelli. 2000. Trypanosoma cruzi: cloning and characterization of a RAB7 gene. Exp. Parasitol. 96:23-31. [PubMed]
178. Lee, M. G., F. T. Yen, Y. Zhang, and B. E. Bihain. 1999. Acquisition of lipoproteins in the procyclic form of Trypanosoma brucei. Mol. Biochem. Parasitol. 100:153-162. [PubMed]
179. Legare, D., D. Richard, R. Mukhopadhyay, Y. D. Stierhof, B. P. Rosen, A. Haimeur, B. Papadopoulou, and M. Ouellette. 2001. The Leishmania ABC protein PGPA is an intracellular metal-thiol transporter ATPase. J. Biol. Chem. 276:26301-26307. [PubMed]
180. Lemmon, S. K., and L. M. Traub. 2000. Sorting in the endosomal system in yeast and animal cells. Curr. Opin. Cell Biol. 12:457-466. [PubMed]
181. Levine, T. P., C. A. Wiggins, and S. Munro. 2000. Inositol phosphorylceramide synthase is located in the Golgi apparatus of Saccharomyces cerevisiae. Mol. Biol. Cell 11:2267-2281. [PMC free article] [PubMed]
182. Lheureux, M., M. Lheureux, T. Vervoort, N. Van Meirvenne, and M. Steinert. 1979. Immunological purification and partial characterization of varient-specific surface antigen messenger RNA of Trypanosoma brucei. Nucleic Acids Res. 7:595-609. [PMC free article] [PubMed]
183. Ligtenberg, M. J., W. Bitter, R. Kieft, D. Steverding, H. Janssen, J. Calafat, and P. Borst. 1994. Reconstitution of a surface transferrin binding complex in insect form Trypanosoma brucei. EMBO J. 13:2565-2573. [PubMed]
184. Lingnau, A., R. Zufferey, M. Lingnau, and D. G. Russell. 1999. Characterization of tGLP-1, a Golgi and lysosome-associated, transmembrane glycoprotein of African trypanosomes. J. Cell Sci. 112:3061-3070. [PubMed]
185. Lippert, D. N., D. W. Dwyer, F. Li, and R. W. Olafson. 1999. Phosphoglycosylation of a secreted acid phosphatase from Leishmania donovani. Glycobiology 9:627-636. [PubMed]
186. Liu, J., X. Qiao, D. Du, and M. G. Lee. 2000. Receptor-mediated endocytosis in the procyclic form of Trypanosoma brucei. J. Biol. Chem. 275:12032-12040. [PubMed]
187. Liu, X., and K. P. Chang. 1992. The 63-kilobase circular amplicon of tunicamycin-resistant Leishmania amazonensis contains a functional N-acetylglucosamine-1-phosphate transferase gene that can be used as a dominant selectable marker in transfection. Mol. Cell. Biol. 12:4112-4122. [PMC free article] [PubMed]
188. Low, P., G. Dallner, S. Mayor, S. Cohen, B. T. Chait, and A. K. Menon. 1991. The mevalonate pathway in the bloodstream form of Trypanosoma brucei. Identification of dolichols containing 11 and 12 isoprene residues. J. Biol. Chem. 266:19250-19257. [PubMed]
189. Lu, H. G., L. Zhong, K. P. Chang, and R. Docampo. 1997. Intracellular Ca2+ pool content and signaling and expression of a calcium pump are linked to virulence in Leishmania mexicana amazonesis amastigotes. J. Biol. Chem. 272:9464-9473. [PubMed]
190. Lu, H. G., L. Zhong, W. de Souza, M. Benchimol, S. Moreno, and R. Docampo. 1998. Ca2+ content and expression of an acidocalcisomal calcium pump are elevated in intracellular forms of Trypanosoma cruzi. Mol. Cell. Biol. 18:2309-2323. [PMC free article] [PubMed]
191. Ma, D. Q., D. G. Russell, S. M. Beverley, and S. J. Turco. 1997. Golgi GDP-mannose uptake requires Leishmania Lpg2—a member of a eukaryotic family of putative nucleotide-sugar transporters. J. Biol. Chem. 272:3799-3805. [PubMed]
192. Maeda, Y., R. Watanabe, C. L. Harris, Y. Hong, K. Ohishi, K. Kinoshita, and T. Kinoshita. 2001. PIG-M transfers the first mannose to glycosylphosphatidylinositol on the lumenal side of the ER. EMBO J. 20:250-261. [PubMed]
193. Magez, S., M. Radwanska, B. Stijlemans, H. Van Xong, E. Pays, and P. De Baetselier. 2001. A conserved flagellar pocket exposed high mannose moiety is used by African trypanosomes as a host cytokine binding molecule. J. Biol. Chem. 276:33258-33564. [PubMed]
194. Maier, A. G., S. Schulreich, M. Bremer, and C. Clayton. 2000. Binding of coatomer by PEX11 C-terminus is not required for function. FEBS Lett. 484:82-86. [PubMed]
195. Maier, A. G., H. Webb, M. Ding, M. Bremser, M. Carrington, and C. Clayton. 2001. The coatomer of Trypanosoma brucei. Mol. Biochem. Parasitol. 115:55-61. [PubMed]
196. Mayor, S., A. K. Menon, and G. A. Cross. 1992. Galactose-containing glycosylphosphatidylinositols in Trypanosoma brucei. J. Biol. Chem. 267:754-761. [PubMed]
197. Mayor, S., A. K. Menon, and G. A. Cross. 1991. Transfer of glycosyl-phosphatidylinositol membrane anchors to polypeptide acceptors in a cell-free system. J. Cell Biol. 114:61-71. [PMC free article] [PubMed]
198. McConnell, J., A. M. Gurnett, J. S. Cordingley, J. E. Walker, and M. J. Turner. 1981. Biosynthesis of Trypanosoma brucei variant surface glycoprotein. I. synthesis, size, and processing of an N-terminal signal peptide. Mol. Biochem. Parasitol. 4:225-242. [PubMed]
199. McConville, M. J., and A. Bacic. 1989. A family of glycoinositol phospholipids from Leishmania major. Isolation, characterization and antigenicity. J. Biol. Chem. 264:757-766. [PubMed]
200. McConville, M. J., and J. M. Blackwell. 1991. Developmental changes in the glycosylated phosphatidylinositols of Leishmania donovani. Characterization of the promastigote and amastigote glycolipids. J. Biol. Chem. 266:15170-15179. [PubMed]
201. McConville, M. J., T. A. C. Collidge, M. A. J. Ferguson, and P. Schneider. 1993. The glycoinositol phospholipids of Leishmania mexicana promastigotes—evidence for the presence of three distinct pathways of glycolipid biosynthesis. J. Biol. Chem. 268:15595-15604. [PubMed]
202. McConville, M. J., and M. A. J. Ferguson. 1993. The structure, biosynthesis and function of glycosylated phosphatidylinositols in the parasitic protozoa and higher eukaryotes. Biochem. J. 294:305-324. [PubMed]
203. McConville, M. J., S. W. Homans, J. E. Thomas-Oates, A. Dell, and A. Bacic. 1990. Structures of the glycoinositolphospholipids from Leishmania major. A family of novel galactofuranose-containing glycolipids. J. Biol. Chem. 265:7385-7394. [PubMed]
204. McConville, M. J., and A. K. Menon. 2000. Recent developments in the cell biology and biochemistry of glycosylphosphatidylinositol lipids. Mol. Membr. Biol. 17:1-16. [PubMed]
205. McConville, M. J., L. F. Schnur, C. Jaffe, and P. Schneider. 1995. Structure of Leishmania lipophosphoglycan-inter- and intra-specific polymorphism in Old World species. Biochem. J. 310:807-818. [PubMed]
206. McConville, M. J., S. J. Turco, M. A. Ferguson, and D. L. Sacks. 1992. Developmental modification of lipophosphoglycan during the differentiation of Leishmania major promastigotes to an infectious stage. EMBO J. 11:3593-3600. [PubMed]
207. McDowell, M. A., D. M. Ransom, and J. D. Bangs. 1998. Glycosylphosphatidylinositol-dependent secretory transport in Trypanosoma brucei. Biochem. J. 335:681-689. [PubMed]
208. McKerrow, J. H. 1999. Development of cysteine protease inhibitors as chemotherapy for parasitic diseases: insights on safety, target validation, and mechanism of action. Int. J. Parasitol. 29:833-837. [PubMed]
209. Mehlert, A., A. Treumann, and M. A. J. Ferguson. 1999. Trypanosoma brucei GPEET-PARP is phosphorylated on six out of seven threonine residues. Mol. Biochem. Parasitol. 98:291-296. [PubMed]
210. Mehlert, A., N. Zitzmann, J. M. Richardson, A. Treumann, and M. A. J. Ferguson. 1998. The glycosylation of the variant surface glycoproteins and procyclic acidic repetitive proteins of Trypanosoma brucei. Mol. Biochem. Parasitol. 91:145-152. [PubMed]
211. Mehul, B., and C. Hughes. 1997. Plasma membrane targetting, vesicular budding and release of galactin 3 from the cytoplasm of mammalian cells during secretion. J. Cell Sci. 110:1169-1178. [PubMed]
212. Mengeling, B. J., S. M. Beverley, and S. J. Turco. 1997. Designing glycoconjugate biosynthesis for an insidious intent: phosphoglycan assembly in Leishmania parasites. Glycobiology 7:873-880. [PubMed]
213. Mensa-Wilmot, K., N. Garg, B. S. McGwire, H. G. Lu, L. Zhong, D. A. Armah, J. H. LeBowitz, and K. P. Chang. 1999. Roles of free GPIs in amastigotes of Leishmania. Mol. Biochem. Parasitol. 99:103-116. [PubMed]
214. Mensa-Wilmot, K., J. H. LeBowitz, K. P. Chang, A. al-Qahtani, B. S. McGwire, S. Tucker, and J. C. Morris. 1994. A glycosylphosphatidylinositol (GPI)-negative phenotype produced in Leishmania major by GPI phospholipase C from Trypanosoma brucei: topography of two GPI pathways. J. Cell Biol. 124:935-947. [PMC free article] [PubMed]
215. Merello, S., M. T. Xavier, and A. J. Parodi. 1994. Novel (rhamnose and ribosyl) and uncommon (xylosyl) monosaccharide residues are present in asparagine-linked oligosaccharide of the trypanosomatid Blastocrithidia culicis. J. Biol. Chem. 269:20294-20298. [PubMed]
216. Milne, K. G., M. A. J. Ferguson, and P. T. Englund. 1999. A novel glycosylphosphatidylinositol in African trypanosomes; a possible catabolic intermediate. J. Biol. Chem. 274:1465-1471. [PubMed]
217. Miranda, K., M. Benchimol, R. Docampo, and W. de Souza. 2000. The fine structure of acidocalcisomes in Trypanosoma cruzi. Parasitol. Res. 86:373-384. [PubMed]
218. Moody, S. F., E. Handman, M. J. McConville, and A. Bacic. 1993. The structure of Leishmania major amastigote lipophosphoglycan. J. Biol. Chem. 268:18457-18466. [PubMed]
219. Moody-Haupt, S., J. H. Patterson, D. Mirelman, and M. J. McConville. 2000. The major surface antigens of Entamoeba histolytica trophozoites are GPI-anchored proteophosphoglycans. J. Mol. Biol. 297:409-420. [PubMed]
220. Morgado-Diaz, J. A., C. V. Nakamura, O. A. Agrellos, W. B. Dias, J. O. Previato, L. Mendonca-Previato, and W. De Souza. 2001. Isolation and characterization of the Golgi complex of the protozoan Trypanosoma cruzi. Parasitology 123:33-43. [PubMed]
221. Morgan, G. W., C. L. Allen, T. R. Jeffries, M. Hollinshead, and M. C. Field. 2001. Developmental and morphological regulation of clathrin-mediated endocytosis in Trypanosoma brucei. J. Cell Sci. 114:2605-2615. [PubMed]
222. Morita, Y. S., A. Acosta-Serrano, L. U. Buxbaum, and P. T. Englund. 2000. Glycosyl phosphatidylinositol myristoylation in African trypanosomes. New intermediates in the pathway for fatty acid remodeling. J. Biol. Chem. 275:14147-14154. [PubMed]
223. Morita, Y. S., K. S. Paul, and P. T. Englund. 2000. Specialized fatty acid synthesis in African trypanosomes: myristate for GPI anchors. Science 288:140-143. [PubMed]
224. Moss, J. M., G. E. Reid, K. A. Mullin, J. L. Zawadzki, R. J. Simpson, and M. J. McConville. 1999. Characterization of a novel GDP-mannose:serine-protein mannose-l-phosphotransferase from Leishmania mexicana. J. Biol. Chem. 274:6678-6688. [PubMed]
225. Mukherjee, T., D. Mandeal, and A. Bhaduri. 2001. Leishmania plasma membrane Mg2+-ATPase is a H+/K+-antiporter involved in glucose symport. Studies with sealed ghosts and vesicles of opposite polarity. J. Biol. Chem. 276:5563-5569. [PubMed]
226. Mullin, K. A., B. Foth, S. M. Ilgoutz, J. Callaghan, G. M. McFadden, and M. J. McConville. 2001. Regulated degradation of ER membrane proteins in a novel tubular lysosome in Leishmania mexicana. Mol. Biol. Cell 12:2364-2377. [PMC free article] [PubMed]
227. Muniz, M., P. Morsomme, and H. Riezman. 2001. Protein sorting upon exit from the endoplasmic reticulum. Cell 104:313-320. [PubMed]
228. Muniz, M., and H. Riezman. 2000. Intracellular transport of GPI-anchored proteins. EMBO J. 19:10-15. [PubMed]
229. Muskus, C., I. Segura, R. Oddone, S. J. Turco, D. A. Leiby, L. Toro, S. Robledo, and N. G. Saravia. 1997. Carbohydrate and LPG expression in Leishmania viannia subgenus. J. Parasitol. 83:671-678. [PubMed]
230. Nagamune, K., T. Nozaki, Y. Maeda, K. Ohishi, T. Fukuma, T. Hara, R. T. Schwarz, C. Sutterlin, R. Brun, H. Riezman, and T. Kinoshita. 2000. Critical roles of glycosylphosphatidylinositol for Trypanosoma brucei. Proc. Natl. Acad. Sci. USA 97:10336-10341. [PubMed]
231. Najib, M. A., N. M. el-Sayed, and J. E. Donelson. 1997. African trypanosmes have differentially expressed genes encoding homologues of the Leishmania GP63 surface protease. J. Biol. Chem. 272:26742-26748. [PubMed]
232. Nandan, D., C. W. Wells, D. Ndegwa, and T. W. Pearson. 1995. Identification of a 44 kDa protein localized within the endoplasmic reticulum of Trypanosoma brucei brucei. Parasitology 111:313-323. [PubMed]
233. Ng, K., E. Handman, and A. Bacic. 1994. Biosynthesis of lipophosphoglycan from Leishmania major: characterization of β(1-3)-galactosyltransferase(s). Glycobiology 4:845-853. [PubMed]
234. Ng, K., E. Handman, and A. Bacic. 1996. Biosynthesis of lipophosphoglycan from Leishmania major: solubilization and characterization of a (β1-3)-galactosyltransferase. Biochem. J. 317:247-255. [PubMed]
235. Ngo, H. M., H. C. Hoppe, and K. A. Joiner. 2000. Differential sorting and post-secretory targeting of proteins in parasitic invasion. Trends Cell Biol. 10:67-72. [PubMed]
236. Nichols, B. J., and H. R. B. Pelham. 1998. SNAREs and membrane fusion in the Golgi apparatus. Biochim. Biophys. Acta 1404:9-31. [PubMed]
237. Nolan, D. P., M. Geuskens, and E. Pays. 1999. N-linked glycans containing linear poly-N-acetyllactosamine as sorting signals in endocytosis in Trypanosoma brucei. Curr. Biol. 9:1169-1172. [PubMed]
238. Nolan, D. P., D. G. Jackson, M. J. Biggs, E. D. Brabazon, A. Pays, F. Van Laethem, F. Paturiaux-Hanocq, J. F. Elliot, H. P. Voorheis, and E. Pays. 2000. Characterization of a novel alanine-rich protein located in surface microdomains in Trypanosoma brucei. J. Biol. Chem. 275:4072-4080. [PubMed]
239. Nolan, D. P., D. G. Jackson, H. J. Windle, A. Pays, M. Geuskens, A. Michel, H. P. Voorheis, and E. Pays. 1997. Characterization of a novel, stage-specific, invariant surface protein in Trypanosoma brucei containing an internal, serine-rich, repetitive motif. J. Biol. Chem. 272:29212-29221. [PubMed]
240. Norris, K. A., J. E. Schrimpf, and M. J. Szabo. 1997. Identification of the gene family encoding the 160-kilodalton Trypanosoma cruzi complement regulatory protein. Infect. Immun. 65:349-357. [PMC free article] [PubMed]
241. Nozaki, T., P. A. Haynes, and G. A. Cross. 1996. Characterization of the Trypanosoma brucei homologue of a Trypanosoma cruzi flagellum-adhesion glycoprotein. Mol. Biochem. Parasitol. 82:245-255. [PubMed]
242. O'Beirne, C., C. M. Lowry, and P. H. Voorheis. 1998. Both IgM and IgG anti-VSG antibodies intiate a cycle of aggregation-disaggregation of bloodstream forms of Trypanosoma brucei without damage to the parasite. Mol. Biochem. Parasitol. 91:165-193. [PubMed]
243. Ochatt, C. M., P. Butikofer, M. Navarro, E. Wirtz, M. Boschung, D. Armah, and G. A. Cross. 1999. Conditional expression of glycosylphosphatidylinositol phospholipase C in Trypanosoma brucei. Mol. Biochem. Parasitol. 103:35-48. [PubMed]
244. Odorizzi, G., M. Babst, and S. D. Emr. 1998. Fab1p PtdIns(3)P 5-kinase function essential for protein sorting in the multivesicular body. Cell 95:847-858. [PubMed]
245. Ohishi, K., N. Inoue, and T. Kinoshita. 2001. PIG-S and PIG-T, essential for GPI anchor attachment to proteins, form a complex with GAA1 and GPI8. EMBO J. 20:4088-4098. [PubMed]
246. Okenu, D. M., K. N. Opara, R. I. Nwuba, and M. Nwagwu. 1999. Purification and characterisation of an extracellularly released protease of Trypanosoma brucei. Parasitol. Res. 85:424-428. [PubMed]
247. Okuda, K., M. Esteva, E. L. Segura, and A. T. Bijovsky. 1999. The cytostome of Trypanosoma cruzi epimastigotes is associated with the flagellar complex. Exp. Parasitol. 92:223-231. [PubMed]
248. Olafson, R. W., J. R. Thomas, M. A. J. Ferguson, R. A. Dwek, M. Chaudhuri, K.-P. Chang, and T. W. Rademacher. 1990. Structures of the N-linked oligosaccharides of gp63, the major surface glycoprotein, from Leishmania mexicana amazonensis. J. Biol. Chem. 265:12240-12247. [PubMed]
249. Overath, P., and T. Aebischer. 1999. Antigen presentation by macrophages harboring intravesicular pathogens. Parasitol. Today 15:325-332. [PubMed]
250. Overath, P., Y.-D. Stierhof, and M. Weise. 1997. Endocytosis and secretion in trypanosomatid parasites—tumultuous traffic in a pocket. Trends Cell Biol. 7:27-33. [PubMed]
251. Paindavoine, P., S. Rolin, S. Van Assel, M. Geuskens, J. C. Jauniaux, C. Dinsart, G. Huet, and E. Pays. 1992. A gene from the variant surface glycoprotein expression site encodes one of several transmembrane adenylate cyclases located on the flagellum of Trypanosoma brucei. Mol. Cell Biol. 12:1218-1225. [PMC free article] [PubMed]
251a. Pal, A., B. S. Hall, D. N. Nesbeth, H. I. Field, and M. C. Field. Differential endocytic functions of Trypanosoma brucei Rab5 isoforms reveal a GPI-specific endosomal pathway. J. Biol. Chem., in press. [PubMed]
252. Parodi, A. J. 1993. N-glycosylation in trypanosomatid protozoa. Glycobiology 3:193-199. [PubMed]
253. Parodi, A. J. 1999. Reglucosylation of glycoprotein and quality control of glycoprotein folding in the endoplasmic reticulum of yeast cells. Biochim. Biophys. Acta 1426:287-295. [PubMed]
254. Parodi, A. J. 2000. Role of N-oligosaccharide endoplasmic reticulum processing reactions in glycoprotein folding and degradation. Biochem. J. 348:1-13. [PubMed]
255. Parodi, A. J., C. Labriola, and J. J. Cazzulo. 1995. The presence of complex-type oligosaccharides at the C-terminal domain glycosylation site of some molecules of cruzipain. Mol. Biochem. Parasitol. 69:247-255. [PubMed]
256. Paturiaux-Hanocq, F., J. Hanocq-Quertier, M. L. de Almeida, D. P. Nolan, A. Pays, L. Vanhamme, J. Van den Abbeele, C. L. Wasunna, M. Carrington, and E. Pays. 2000. A role for the dynamic acylation of a cluster of cysteine residues in regulating the activity of the glycosylphosphatidylinositol-specific phospholipase C of Trypanosoma brucei. J. Biol. Chem. 275:12147-12155. [PubMed]
257. Paturiaux-Hanocq, F., N. Zitzmann, J. Hanocq-Quertier, L. Vanhamme, S. Rolin, M. Geuskens, M. A. Ferguson, and E. Pays. 1997. Expression of a variant surface glycoprotein of Trypanosoma gambiense in procyclic forms of Trypanosoma brucei shows that the cell type dictates the nature of the glycosylphosphatidylinositol membrane anchor attached to the glycoprotein. Biochem. J. 324:885-895. [PubMed]
258. Paul, K. S., D. Jiang, Y. S. Morita, and P. T. Englund. 2001. Fatty acid synthesis in African trypanosomes: a solution to the myristate mystery. Trends Parasitol. 17:381-387. [PubMed]
259. Pays, E., and D. P. Nolan. 1998. Expression and function of surface proteins in Trypanosoma brucei. Mol. Biochem. Parasitol. 91:3-36. [PubMed]
260. Pazour, G. J., C. G. Wilkerson, and G. B. Witman. 1998. A dynein light chain is essential for the retrograde particle movement of intraflagellar transport (IFT). J. Cell Biol. 141:979-992. [PMC free article] [PubMed]
261. Pereira-Chioccola, V. L., A. Acosta-Serrano, I. Correia De Almeida, M. A. Ferguson, T. Souto-Padron, M. M. Rodrigues, L. R. Travassos, and S. Schenkman. 2000. Mucin-like molecules form a negatively charged coat that protects Trypanosoma cruzi trypomastigotes from killing by human anti-α-galactosyl antibodies. J. Cell Sci. 113:1299-1307. [PubMed]
262. Peters, C., M. Kawakami, M. Kaul, T. Ilg, P. Overath, and T. Aebischer. 1997. Secreted proteophosphoglycan of Leishmania mexicana amastigotes activates complement by triggering the mannan binding lectin pathway. Eur. J. Immunol. 27:2666-2672. [PubMed]
263. Piani, A., T. Ilg, A. G. Elefanty, J. Curtis, and E. Handman. 1999. Leishmania major proteophosphoglycan is expressed by amastigotes and has an immunomodulatory effect on macrophage function. Microbes Infect. 1:589-599. [PubMed]
264. Pimenta, P. F., and W. De Souza. 1985. Fine structure and cytochemistry of the endoplasmic reticulum and its association with the plasma membrane of Leishmania mexicana amazonensis. J. Submicrosc. Cytol. 17:413-419. [PubMed]
265. Pimenta, P. F., E. M. Saraiva, and D. L. Sacks. 1991. The comparative fine structure and surface glycoconjugate expression of three life stages of Leishmania major. Exp. Parasitol. 72:191-204. [PubMed]
266. Piper, R. C., X. W. Xu, D. G. Russell, B. M. Little, and S. M. Landfear. 1995. Differential targeting of two glucose transporters from Leishmania enriettii is mediated by an NH2-terminal domain. J. Cell Biol. 128:499-508. [PMC free article] [PubMed]
267. Polishchuk, R. S., E. V. Polishchuk, P. Marra, S. Alberti, R. Buccione, A. Luini, and A. A. Mironov. 2000. Correlative light-electron microscopy reveals the tubular-saccular ultrastructure of carrier operating between Golgi apparatus and plasma membrane. J. Cell Biol. 148:45-58. [PMC free article] [PubMed]
268. Pollevick, G. D., J. M. Di Noia, M. L. Salto, C. Lima, M. S. Leguizamon, R. M. de Lederkremer, and A. C. Frasch. 2000. Trypanosoma cruzi surface mucins with exposed variant epitopes. J. Biol. Chem. 275:27671-27680. [PubMed]
269. Pontes de Carvalho, L. C., S. Tomlinson, F. Vandekerckhove, E. J. Bienen, A. B. Clarkson, M.-S. Jiang, G. W. Hart, and V. Nussenzweig. 1993. Characterization of a novel trans-sialidase of Trypanosoma brucei procyclic trypomastigotes and identification of procyclin as the main sialic acid acceptor. J. Exp. Med. 177:465-474. [PMC free article] [PubMed]
270. Porto-Carreiro, I., M. Attias, K. Miranda, W. De Souza, and N. Cunha-e-Silva. 2000. Trypanosoma cruzi epimastigote endocytic pathway: cargo enters the cytostome and passes through an early endosomal network before storage in reservosomes. Eur. J. Cell Biol. 79:858-869. [PubMed]
271. Prado-Figueroa, M., J. Raper, and F. R. Opperdoes. 1994. Possible localisation of dolichol-dependent mannosyltransferases of Trypanosoma brucei to the rough endoplasmic reticulum. Mol. Biochem. Parasitol. 63:255-264. [PubMed]
272. Previato, J. O., C. Jones, L. P. Goncalves, R. Wait, L. R. Travassos, and L. Mendonca-Previato. 1994. O-glycosidically linked N-acetylglucosamine-bound oligosaccharides from glycoproteins of Trypanosoma cruzi. Biochem. J. 301:151-159. [PubMed]
273. Previato, J. O., C. Jones, R. Wait, F. Routier, E. Saraiva, and L. Mendonca-Previato. 1997. Leishmania adleri, a lizard parasite, expresses structurally similar glycoinositolphospholipids to mammalian Leishmania. Glycobiology 7:687-695. [PubMed]
274. Previato, J. O., C. Jones, M. T. Xavier, R. Wait, L. R. Travassos, A. J. Parodi, and L. Mendonca-Previato. 1995. Structural characterization of the major glycosylphosphatidylinositol membrane-anchored glycoprotein from epimastigote forms of Trypanosoma cruzi Y-strain. J. Biol. Chem. 270:7241-7250. [PubMed]
275. Previato, J. O., M. Sola-Penna, O. A. Agrellos, C. Jones, T. Oeltmann, L. R. Travassos, and L. Mendonca-Previato. 1998. Biosynthesis of O-N-acetylglucosamine-linked glycans in Trypanosoma cruzi. Characterization of the novel uridine diphospho-N-acetylglucosamine:polypeptide N-acetylglucosaminyltransferase-catalyzing formation of N-acetylglucosamine-α-1-O-threonine. J. Biol. Chem. 273:14982-14988. [PubMed]
276. Proudfoot, L., P. Schneider, M. A. J. Ferguson, and M. J. McConville. 1995. Biosynthesis of the glycolipid anchor of lipophosphoglycan and the structurally related glycoinositolphospholipids from Leishmania major. Biochem. J. 308:45-55. [PubMed]
277. Puentes, S. M., R. P. Da Silva, D. L. Sacks, C. H. Hammer, and K. A. Joiner. 1990. Serum resistance of metacyclic stage Leishmania major promastigotes is due to release of C5b-9. J. Immunol. 145:4311-4316. [PubMed]
278. Ralton, J. E., and M. J. McConville. 1998. Delineation of three pathways of glycosylphosphatidylinositol biosynthesis in Leishmania mexicana—precursors from different pathways are assembled on distinct pools of phosphatidylinositol and undergo fatty acid remodeling. J. Biol. Chem. 273:4245-4257. [PubMed]
279. Ralton, J. E., K. G. Milne, M. L. S. Guther, R. A. Field, and M. A. J. Ferguson. 1993. The mechanism of inhibition of glycosylphosphatidylinositol anchor biosynthesis in Trypanosoma brucei by mannosamine. J. Biol. Chem. 268:24183-24189. [PubMed]
280. Ralton, J. E., K. A. Mullin, and M. J. McConville. Intracellular trafficking of GPI-anchored proteins and free GPIs in Leishmania mexicana. Biochem. J., in press. [PubMed]
281. Rangarajan, D., S. Gokool, M. McCrossan, and D. F. Smith. 1995. The geneB protein localises to the surface of Leishmania major parasites in the absence of metacyclic stage lipophosphoglycan. J. Cell Sci. 108:3359-3366. [PubMed]
282. Redman, C. A., P. Schneider, A. Mehlert, and M. A. J. Ferguson. 1995. The glycoinositol-phospholipids of Phytomonas. Biochem. J. 311:495-503. [PubMed]
283. Reggiori, F., M. W. Black, and H. R. B. Relham. 2000. Polar transmembrane domains target proteins to the interior of the yeast vacuole. Mol. Biol. Cell 11:3737-3749. [PMC free article] [PubMed]
284. Reggiori, F., and A. Conzelmann. 1998. Biosynthesis of inositol phosphoceramides and remodeling of glycosylphosphatidylinositol anchors in Saccharomyces cerevisiae are mediated by different enzymes. J. Biol. Chem. 273:30550-30559. [PubMed]
285. Rivas, L., L. Kahl, K. Manson, and D. McMahon-Pratt. 1991. Biochemical characterization of the protective membrane glycoprotein GP46/M-2 of Leishmania amazonensis. Mol. Biochem. Parasitol. 47:235-243. [PubMed]
286. Robinson, D. R., T. Sherwin, A. Ploubidou, E. H. Byard, and K. Gull. 1995. Microtubule polarity and dynamics in the control of organelle positioning, segregation, and cytokinesis in the trypanosome cell cycle. J. Cell Biol. 128:1163-1172. [PMC free article] [PubMed]
287. Roditi, I., A. Furger, S. Ruepp, N. Schurch, and P. Bütikofer. 1998. Unravelling the procyclin coat of Trypanosoma brucei. Mol. Biochem. Parasitol. 91:117-130. [PubMed]
288. Rodrigues, C. O., D. A. Scott, and R. Docampo. 1999. Presence of a vacuolar H+-pyrophosphatase in promastigotes of Leishmania donovani and its localization to a different compartment from the vacuolar H+-ATPase. Biochem. J. 340:759-766. [PubMed]
289. Roggy, J. L., and J. D. Bangs. 1999. Molecular cloning and biochemical characterization of a VCP homolog in African trypanosomes. Mol. Biochem. Parasitol. 98:1-15. [PubMed]
290. Rout, M. P., and M. C. Field. 2001. Isolation and characterization of subnuclear compartments from Trypanosoma brucei. Identification of a major repetitive nuclear lamina component. J. Biol. Chem. 276:38261-38271. [PubMed]
291. Routier, F. H., A. P. Hidson, I. A. Ivanova, A. J. Ross, Y. E. Tsvetkov, D. V. Yashunsky, P. A. Bates, A. V. Nikolaev, and M. A. J. Ferguson. 2000. Characterization of the elongating α-D-mannosyl phosphate transferase from three species of Leishmania using synthetic acceptor substrate analogues. Biochemistry 39:8017-8025. [PubMed]
292. Ruiz, F. A., N. Marchesini, M. Seufferheld, Govindjee, and R. Docampo. 2001. The polyphosphate bodies of Chlamydomonas reinhardtii possess a proton-pumping pyrophosphatase and are similar to acidocalcisomes. J. Biol. Chem. 276:46196-46203. [PubMed]
293. Ruiz, F. A., C. O. Rodriguez, and R. Docampo. 2001. Rapid changes in polyphosphate content within acidocalcisomes in response to cell growth, differentiation and environmental stress in Trypanosoma cruzi. J. Biol. Chem. 276:26114-26121. [PubMed]
294. Ruiz-Moreno, L., A. T. Bijovsky, J. Pudles, M. J. Alves, and W. Colli. 1995. Trypanosoma cruzi: monoclonal antibody to cytoskeleton recognizes giant proteins of the flagellar attachment zone. Exp. Parasitol. 80:605-615. [PubMed]
295. Russell, D. G. 1994. Biology of the Leishmania surface—with particular reference to the surface proteinase, GP63. Protoplasma 181:191-201.
296. Sacks, D. L. 2001. Leishmania-sand fly interactions controlling species-specific vector competence. Cell. Microbiol. 3:189-196. [PubMed]
297. Sacks, D. L., G. Modi, E. Rowton, G. Spath, L. Epstein, S. J. Turco, and S. M. Beverley. 2000. The role of phosphoglycans in Leishmania-sand fly interactions. Proc. Natl. Acad. Sci. USA 97:406-411. [PubMed]
298. Salmon, D., M. Geuskens, F. Hanocq, J. Hanocq-Quertier, D. Nolan, L. Ruben, and E. Pays. 1994. A novel heterodimeric transferrin receptor encoded by a pair of VSG expression site-associated genes in T. brucei. Cell 78:75-86. [PubMed]
299. Sanchez, M. A., B. Ullman, S. M. Landfear, and N. S. Carter. 1999. Cloning and functional expression of a gene encoding a P1 type nucleoside transporter from Trypanosoma brucei. J. Biol. Chem. 274:30244-30249. [PubMed]
300. Sanchez, M. A., D. Zeoli, E. M. Klamo, M. P. Kavanaugh, and S. M. Landfear. 1995. A family of putative receptor-adenylate cyclases from Leishmania donovani. J. Biol. Chem. 270:17551-17558. [PubMed]
301. Saraiva, E. M., P. F. Pimenta, T. N. Brodin, E. Rowton, G. B. Modi, and D. L. Sacks. 1995. Changes in lipophosphoglycan and gene expression associated with the development of Leishmania major in Phlebotomus papatasi. Parasitology 111:275-287. [PubMed]
302. Schell, D., Y. D. Stierhof, and P. Overath. 1990. Purification and characterization of a tartrate-sensitive acid phosphatase of Trypanosoma brucei. FEBS Lett. 271:67-70. [PubMed]
303. Schenkman, S., D. Eichinger, M. E. Pereira, and V. Nussenzweig. 1994. Structural and functional properties of Trypanosoma cruzi trans-sialidase. Annu. Rev. Microbiol. 48:499-523. [PubMed]
304. Schenkman, S., M. A. J. Ferguson, N. Heise, M. L. C. Dealmeida, R. A. Mortara, and N. Yoshida. 1993. Mucin-like glycoproteins linked to the membrane by glycosylphosphatidylinositol anchor are the major acceptors of sialic acid in a reaction catalyzed by trans-sialidase in metacyclic forms of Trypanosoma cruzi. Mol. Biochem. Parasitol. 59:293-303. [PubMed]
305. Schneider, A., W. Eichenberger, and T. A. Seebeck. 1988. A microtubule-binding protein of Trypanosoma brucei which contain covalently bound fatty acid. J. Biol. Chem. 263:6472-6475. [PubMed]
306. Schneider, P., M. A. Ferguson, M. J. McConville, A. Mehlert, S. W. Homans, and C. Bordier. 1990. Structure of the glycosyl-phosphatidylinositol membrane anchor of the Leishmania major promastigote surface protease. J. Biol. Chem. 265:16955-16964. [PubMed]
307. Schneider, P., M. J. McConville, and M. A. J. Ferguson. 1994. Characterization of GDP-α-D-arabinopyranose, the precursor of D-Arap in Leishmania major lipophosphoglycan. J. Biol. Chem. 269:18332-18337. [PubMed]
308. Schneider, P., J. P. Rosat, A. Ransijn, M. A. J. Ferguson, and M. J. McConville. 1993. Characterization of glycoinositol phospholipids in the amastigote stage of the protozoan parasite Leishmania major. Biochem. J. 295:555-564. [PubMed]
309. Schneider, P., L. F. Schnur, C. L. Jaffe, M. A. J. Ferguson, and M. J. McConville. 1994. Glycoinositol-phospholipid profiles of four serotypically distinct Old World Leishmania strains. Biochem. J. 304:603-609. [PubMed]
310. Schneider, P., A. Treumann, K. G. Milne, M. J. McConville, N. Zitzmann, and M. A. J. Ferguson. 1996. Structural studies on a lipoarabinogalactan of Crithidia fasciculata. Biochem. J. 313:963-971. [PubMed]
311. Scott, D. A., W. de Souza, M. Benchimol, L. Zhong, H.-G. Lu, S. N. Moreno, and R. Docampo. 1998. Presence of a plant-like proton-pumping pyrophosphatase in acidocalcisomes of Trypanosoma cruzi. J. Biol. Chem. 273:22151-22158. [PubMed]
312. Scott, D. A., and R. Docampo. 1998. Two types of H+-ATPase are involved in the acidification of internal compartments in Trypanosoma cruzi. Biochem. J. 331:583-589. [PubMed]
313. Scott, D. A., R. Docampo, J. A. Dvorak, S. Shi, and R. D. Leapman. 1997. In situ compositional analysis of acidocalcisomes in Trypanosoma cruzi. J. Biol. Chem. 272:28020-28029. [PubMed]
314. Seaman, M. N., J. M. McCaffery, and S. D. Emr. 1998. A membrane coat complex essential for endosome-to-Golgi retrograde transport in yeast. J. Cell Biol. 142:665-681. [PMC free article] [PubMed]
315. Selzer, P. M., S. Pingel, I. Hsieh, B. Ugele, V. J. Chan, J. C. Engel, M. Bogyo, D. G. Russell, J. A. Sakanari, and J. H. McKerrow. 1999. Cysteine protease inhibitors as chemotherapy: lessons from a parasite target. Proc. Natl. Acad. Sci. USA 96:11015-11022. [PubMed]
316. Semenza, J. C., K. G. Hardwick, N. Dean, and H. R. B. Pelham. 1990. ERD2, a yeast gene required for the receptor-mediated retrieval of luminal ER proteins from the secretory pathway. Cell 61:1349-1357. [PubMed]
317. Sevlever, D., K. J. Mann, and M. E. Medof. 2001. Differential effect of 1,10-phenanthroline on mammalian, yeast, and parasite glycosylphosphatidylinositol anchor synthesis. Biochem. Biophys. Res. Commun. 288:1112-1118. [PubMed]
318. Seyfang, A., D. Mecke, and M. Duszenko. 1990. Degradation, recycling, and shedding of Trypanosoma brucei variant surface glycoprotein. J. Protozool. 37:546-552. [PubMed]
319. Shakarian, A. M., and D. M. Dwyer. 2000. Pathogenic Leishmania secrete antigenically related chitinases which are encoded by a highly conserved gene locus. Exp. Parasitol. 94:238-242. [PubMed]
320. Shapiro, S. Z., and P. Webster. 1989. Coated vesicles from the protozoan parasite Trypanosoma brucei: purification and characterization. J. Protozool. 36:344-349. [PubMed]
321. Sharma, D. K., J. D. Hilley, J. D. Bangs, G. H. Coombs, J. C. Mottram, and A. K. Menon. 2000. Soluble GPI8 restores glycosylphosphatidylinositol anchoring in a trypanosome cell-free system depleted of lumenal endoplasmic reticulum proteins. Biochem. J. 351:717-722. [PubMed]
322. Sharma, D. K., J. Vidugiriene, J. D. Bangs, and A. K. Menon. 1999. A cell-free assay for glycosylphosphatidylinositol anchoring in African trypanosomes—demonstration of a transamidation reaction mechanism. J. Biol. Chem. 274:16479-16486. [PubMed]
323. Shimamura, M., K. M. Hager, and S. L. Hajduk. 2001. The lysosomal targeting and intracellular metabolism of trypanosome lytic factor by Trypanosoma brucei brucei. Mol. Biochem. Parasitol. 115:227-237. [PubMed]
324. Sibley, L. D., and N. W. Andrews. 2000. Cell invasion by un-palatable parasites. Traffic 1:100-106. [PubMed]
325. Smith, A. C., M. J. Paterson, A. Crossman, J. S. Brimacombe, and M. A. J. Ferguson. 2000. Parasite-specific inhibition of the glycosylphosphatidylinositol biosynthetic pathway by stereoisomeric substrate analogues. Biochemistry 39:11801-11807. [PubMed]
326. Smith, D. F., and D. Rangarajan. 1995. Cell surface components of Leishmania: identification of a novel parasite lectin. Glycobiology 5:161-166. [PubMed]
327. Smith, T. K., A. Crossman, C. N. Borissow, M. J. Paterson, A. Dix, J. S. Brimacombe, and M. A. Ferguson. 2001. Specificity of GlcNAc-PI de-N-acetylase of GPI biosynthesis and synthesis of parasite-specific suicide substrate inhibitors. EMBO J. 20:3322-3332. [PubMed]
328. Smith, T. K., F. C. Milne, D. K. Sharma, A. Crossman, J. S. Brimacombe, and M. A. J. Ferguson. 1997. Early steps in glycosylphosphatidylinositol biosynthesis in Leishmania major. Biochem. J. 326:393-400. [PubMed]
329. Smith, T. K., D. K. Sharma, A. Crossman, J. S. Brimacombe, and M. A. J. Ferguson. 1999. Selective inhibitors of the glycosylphosphatidylinositol biosynthetic pathway of Trypanosoma brucei. EMBO J. 18:5922-5930. [PubMed]
330. Snapp, E. L., and S. M. Landfear. 1999. Characterization of a targeting motif for the flagellar membrane protein in Leishmania enriettii. J. Biol. Chem. 274:29543-29548. [PubMed]
331. Snapp, E. L., and S. M. Landfear. 1997. Cytoskeletal association is important for differential targeting of glucose transporter isoforms in Leishmania. J. Cell Biol. 139:1775-1783. [PMC free article] [PubMed]
332. Soares, M. J., T. Souto-Padron, and W. De Souza. 1992. Identification of a large pre-lysosomal compartment in the pathogenic protozoon Trypanosoma cruzi. J. Cell Sci. 102:157-167. [PubMed]
333. Souto-Padron, T., W. de Souza, and J. E. Heuser. 1984. Quick-freeze, deep-etch rotary replication of Trypanosoma cruzi and Herpetomonas megaseliae. J. Cell Sci. 69:167-178. [PubMed]
334. Souza, D. W., D. T. U. Carvalho, and M. Benchimol. 1978. Trypanosoma cruzi: ultrastructural, cytochemical and freeze-fracture studies of protein uptake. Exp. Parasitol. 45:101-115. [PubMed]
335. Spath, G. F., L. Epstein, B. Leader, S. M. Singer, H. A. Avila, S. J. Turco, and S. M. Beverley. 2000. Lipophosphoglycan is a virulence factor distinct from related glycoconjugates in the protozoan parasite Leishmania major. Proc. Natl. Acad. Sci. USA 97:9258-9263. [PubMed]
336. Springer, S., A. Spang, and R. Schekman. 1999. A primer on vesicle budding. Cell 97:145-148. [PubMed]
337. Steverding, D., and P. Overath. 1996. Trypanosoma brucei with an active metacyclic variant surface gene expression site expresses a transferrin receptor derived from Esag6 and Esag7. Mol. Biochem. Parasitol. 78:285-288. [PubMed]
338. Steverding, D., Y. D. Stierhof, M. Chaudhri, M. Ligtenberg, D. Schell, A. G. Beck-Sickinger, and P. Overath. 1994. ESAG 6 and 7 products of Trypanosoma brucei form a transferrin binding protein complex. Eur. J. Cell Biol. 64:78-87. [PubMed]
339. Steverding, D., Y. D. Stierhof, H. Fuchs, R. Tauber, and P. Overath. 1995. Transferrin-binding protein complex is the receptor for transferrin uptake in Trypanosoma brucei. J. Cell Biol. 131:1173-1182. [PMC free article] [PubMed]
340. Stierhof, Y. D., P. A. Bates, R. L. Jacobson, M. E. Rogers, Y. Schlein, E. Handman, and T. Ilg. 1999. Filamentous proteophosphoglycan secreted by Leishmania promastigotes forms gel-like three-dimensional networks that obstruct the digestive tract of infected sandfly vectors. Eur. J. Cell Biol. 78:675-689. [PubMed]
341. Stierhof, Y. D., T. Ilg, D. G. Russell, H. Hohenberg, and P. Overath. 1994. Characterization of polymer release from the flagellar pocket of Leishmania mexicana promastigotes. J. Cell Biol. 125:321-331. [PMC free article] [PubMed]
342. Stierhof, Y. D., M. Wiese, T. Ilg, P. Overath, M. Haner, and U. Aebi. 1998. Structure of a filamentous phosphoglycoprotein polymer: the secreted acid phosphatase of Leishmania mexicana. J. Mol. Biol. 282:137-148. [PubMed]
343. Straus, A. H., S. B. Levery, M. G. Jasiulionis, M. E. K. Salyan, S. J. Steele, L. R. Travassos, S. Hakomori, and H. K. Takahashi. 1993. Stage-specific glycosphingolipids from amastigote forms of Leishmania (L.) amazonensis. Immunogenicity and role in parasite binding and invasion of macrophages. J. Biol. Chem. 268:13723-13730. [PubMed]
344. Sutterlin, C., T. L. Doering, F. Schimmoller, S. Schroder, and H. Riezman. 1997. Specific requirements for the ER to Golgi transport of GPI-anchored proteins in yeast. J. Cell Sci. 110:2703-2714. [PubMed]
345. Tambourgi, D. V., T. L. Kipnis, W. D. de Silva, K. A. Joiner, A. Sher, S. Heath, B. F. Hall, and G. B. Ogden. 1993. A partial cDNA clone of trypomastigote decay-accelerating factor (T-DAF), a developmentally regulated complement inhibitor of Trypanosoma cruzi, has genetic and functional similarities to the human complement inhibitor DAF. Infect. Immun. 61:3656-3663. [PMC free article] [PubMed]
346. Teasdale, R. D., and M. R. Jackson. 1996. Signal-mediated sorting of membrane proteins between the endoplasmic reticulum and the Golgi apparatus. Annu. Rev. Cell Dev. Biol. 12:27-54. [PubMed]
347. Teixeira, S. M. R., D. G. Russell, L. V. Kirchhoff, and J. E. Donelson. 1994. A differentially expressed gene family encoding “amastin,” a surface protein of Trypanosoma cruzi amastigotes. J. Biol. Chem. 269:20509-20516. [PubMed]
348. Todeschini, A. R., E. X. da Silveira, C. Jones, R. Wait, J. O. Previato, and L. Mendonca-Previato. 2001. Structure of O-glycosidically linked oligosaccharides from glycoproteins of Trypanosoma cruzi CL-Brener strain: evidence for the presence of O-linked sialyl-oligosaccharides. Glycobiology 11:47-55. [PubMed]
349. Trombetta, E. S., and A. Helenius. 1998. Lectins as chaperones in glycoprotein folding. Curr. Opin. Struct. Biol. 8:587-592. [PubMed]
350. Trowbridge, I. S., J. F. Collawn, and C. R. Hopkins. 1993. Signal-dependent membrane protein trafficking in the endocytic pathway. Annu. Rev. Cell Biol. 9:129-161. [PubMed]
351. Turco, S. J., G. F. Spath, and S. M. Beverley. 2001. Is lipophosphoglycan a virulence factor? A surprising diversity between Leishmania species. Trends Parasitol. 17:223-226. [PubMed]
352. Ueda-Nakamura, T., M. Attias, and W. de Souza. 2001. Megasome biogenesis in Leishmania amazonensis: a morphometric and cytochemical study. Parasitol. Res. 87:89-97. [PubMed]
353. Vannier-Santos, M. A., A. Martiny, U. Lins, J. A. Urbina, V. M. Borges, and W. de Souza. 1999. Impairment of sterol biosynthesis leads to phosphorus and calcium accumulation in Leishmania acidocalcisomes. Microbiology 145:3213-3220. [PubMed]
354. Vassella, E., J. V. Den Abbeele, P. Butikofer, C. K. Renggli, A. Furger, R. Brun, and I. Roditi. 2000. A major surface glycoprotein of Trypanosoma brucei is expressed transiently during development and can be regulated post-transcriptionally by glycerol or hypoxia. Genes Dev. 14:615-626. [PubMed]
355. Vasudevan, G., N. S. Carter, M. E. Drew, S. M. Beverley, M. A. Sanchez, A. Seyfang, B. Ullman, and S. M. Landfear. 1998. Cloning of Leishmania nucleoside transporter genes by rescue of a transport-deficient mutant. Proc. Natl. Acad. Sci. USA 95:9873-9878. [PubMed]
356. Vickerman, K. 1969. The fine structure of Trypanosoma congolense in its bloodstream phase. J. Protozool. 16:54-69. [PubMed]
357. Vickerman, K. 1969. On the surface coat and flagellar adhesion in trypanosomes. J. Cell Sci. 5:163-193. [PubMed]
358. Vidugiriene, J., and A. K. Menon. 1993. Early lipid intermediates in glycosyl-phosphatidylinositol anchor assembly are synthesized in the ER and located in the cytoplasmic leaflet of the ER membrane bilayer. J. Cell Biol. 121:987-996. [PMC free article] [PubMed]
359. Vidugiriene, J., and A. K. Menon. 1994. The GPI anchor of cell-surface proteins is synthesized on the cytoplasmic face of the endoplasmic reticulum. J. Cell Biol. 127:333-341. [PMC free article] [PubMed]
360. Vidugiriene, J., D. K. Sharma, T. K. Smith, N. A. Baumann, and A. K. Menon. 1999. Segregation of glycosylphosphatidylinositol biosynthetic reactions in a subcompartment of the endoplasmic reticulum. J. Biol. Chem. 274:15203-15212. [PubMed]
361. Webster, P. 1989. Endocytosis by African trypanosomes. I. Three-dimensional structure of the endocytic organelles in Trypanosoma brucei and T. congolense. Eur. J. Cell Biol. 49:295-302. [PubMed]
362. Webster, P., and W. R. Fish. 1989. Endocytosis by African trypanosomes. II. Occurrence in different life-cycle stages and intracellular sorting. Eur. J. Cell Biol. 49:303-310. [PubMed]
363. Webster, P., and D. J. Grab. 1988. Intracellular colocalization of variant surface glycoprotein and transferrin-gold in Trypanosoma brucei. J. Cell Biol. 106:279-288. [PMC free article] [PubMed]
364. Webster, P., D. C. Russo, and S. J. Black. 1990. The interaction of Trypanosoma brucei with antibodies to variant surface glycoproteins. J. Cell Sci. 96:249-255. [PubMed]
365. Weise, F., Y. D. Stierhof, C. Kuhn, M. Wiese, and P. Overath. 2000. Distribution of GPI-anchored proteins in the protozoan parasite Leishmania, based on an improved ultrastructural description using high-pressure frozen cells. J. Cell Sci. 113:4587-4603. [PubMed]
366. Wendland, B., S. D. Emr, and H. Riezman. 1998. Protein traffic in the yeast endocytic and vacuolar protein sorting pathways. Curr. Opin. Cell Biol. 10:513-522. [PubMed]
367. Wiese, M., O. Berger, Y. D. Stierhof, M. Wolfram, M. Fuchs, and P. Overath. 1996. Gene cloning and cellular localization of a membrane-bound acid phosphatase of Leishmania mexicana. Mol. Biochem. Parasitol. 82:153-165. [PubMed]
368. Wiese, M., I. Gorcke, and P. Overath. 1999. Expression and species-specific glycosylation of Leishmania mexicana secreted acid phosphatase in Leishmania major. Mol. Biochem. Parasitol. 102:325-329. [PubMed]
369. Wiese, M., T. Ilg, F. Lottspeich, and P. Overath. 1995. Ser/Thr-rich repetitive motifs as targets for phosphoglycan modifications in Leishmania mexicana secreted acid phosphatase. EMBO J. 14:1067-1074. [PubMed]
370. Winter, G., M. Fuchs, M. J. McConville, Y. D. Stierhof, and P. Overath. 1994. Surface antigens of Leishmania mexicana amastigotes-characterization of glycoinositol phospholipids and a macrophage-derived glycosphingolipid. J. Cell Sci. 107:2471-2482. [PubMed]
371. Wolfram, M., T. Ilg, J. C. Mottram, and P. Overath. 1995. Antigen presentation by Leishmania mexicana-infected macrophages: activation of helper T cells specific for amastigote cysteine proteinases requires intracellular killing of the parasites. Eur. J. Immunol. 25:1094-1100. [PubMed]
372. Woods, A. S., A. J. Baines, and K. Gull. 1989. Evidence for a Mr 88,000 glycoprotein with a transmembrane association to a unique flagellum attachment region in Trypanosoma brucei. J. Cell Sci. 93:501-508. [PubMed]
373. Wu, Y., Y. El Fakhry, D. Sereno, S. Tamar, and B. Papadopoulou. 2000. A new developmentally regulated gene family in Leishmania amastigotes encoding a homologue of amastin surface proteins. Mol. Biochem. Parasitol. 110:345-357. [PubMed]
374. Yahiaoui, B., M. Loyens, A. Taibi, R. Schoneck, J. F. Dubremetz, and M. A. Ouaissi. 1993. Characterization of a Leishmania antigen associated with cytoplasmic vesicles resembling an endosomal-like structure. Parasitology 107:497-507. [PubMed]
375. Yang, H., D. G. Russell, B. Zheng, M. Eiki, and M. G. Lee. 2000. Sequence requirements for trafficking of the CRAM transmembrane protein to the flagellar pocket of African trypanosomes. Mol. Cell. Biol. 20:5149-5163. [PMC free article] [PubMed]
376. Zamze, S. 1991. Glycosylation in parasitic protozoa of the trypanosomatidae family. Glycoconjugate J. 8:443-447. [PubMed]
377. Zawadzki, J., C. Scholz, G. Currie, G. H. Coombs, and M. J. McConville. 1998. The glycoinositolphospholipids from Leishmania panamensis contain unusual glycan and lipid moieties. J. Mol. Biol. 282:287-299. [PubMed]
378. Ziegelbauer, K., and P. Overath. 1993. Organization of two invariant surface glycoproteins in the surface coat of Trypanosoma brucei. Infect. Immun. 61:4540-4545. [PMC free article] [PubMed]
379. Zilberstein, D. 1993. Transport of nutrients and ions across membranes of trypanosomatid parasites. Adv. Parasitol. 32:261-291. [PubMed]
380. Zitzmann, N., A. Mehlert, S. Carroue, P. M. Rudd, and M. A. Ferguson. 2000. Protein structure controls the processing of the N-linked oligosaccharides and glycosylphosphatidylinositol glycans of variant surface glycoproteins expressed in bloodstream form Trypanosoma brucei. Glycobiology 10:243-249. [PubMed]

Articles from Microbiology and Molecular Biology Reviews : MMBR are provided here courtesy of American Society for Microbiology (ASM)