PMCCPMCCPMCC

Search tips
Search criteria 

Advanced

 
Logo of mmbrPermissionsJournals.ASM.orgJournalMMBR ArticleJournal InfoAuthorsReviewers
 
Microbiol Mol Biol Rev. Mar 2002; 66(1): 64–93.
PMCID: PMC120782
α-Crystallin-Type Heat Shock Proteins: Socializing Minichaperones in the Context of a Multichaperone Network
Franz Narberhaus*
Institut für Mikrobiologie, Eidgenössische Technische Hochschule, CH-8092 Zürich, Switzerland
*Mailing address: Institut für Mikrobiologie, ETH-Zentrum, Schmelzbergstrasse 7, CH-8092 Zürich, Switzerland. Phone: 41-1-632-2586. Fax: 41-1-632-1148. E-mail: fnarber/at/micro.biol.ethz.ch.
α-Crystallins were originally recognized as proteins contributing to the transparency of the mammalian eye lens. Subsequently, they have been found in many, but not all, members of the Archaea, Bacteria, and Eucarya. Most members of the diverse α-crystallin family have four common structural and functional features: (i) a small monomeric molecular mass between 12 and 43 kDa; (ii) the formation of large oligomeric complexes; (iii) the presence of a moderately conserved central region, the so-called α-crystallin domain; and (iv) molecular chaperone activity. Since α-crystallins are induced by a temperature upshift in many organisms, they are often referred to as small heat shock proteins (sHsps) or, more accurately, α-Hsps. α-Crystallins are integrated into a highly flexible and synergistic multichaperone network evolved to secure protein quality control in the cell. Their chaperone activity is limited to the binding of unfolding intermediates in order to protect them from irreversible aggregation. Productive release and refolding of captured proteins into the native state requires close cooperation with other cellular chaperones. In addition, α-Hsps seem to play an important role in membrane stabilization. The review compiles information on the abundance, sequence conservation, regulation, structure, and function of α-Hsps with an emphasis on the microbial members of this chaperone family.
Our knowledge about protein folding has increased substantially over the last 30 years. The traditional view that proteins fold spontaneously (9) was revised upon the finding that many proteins in a living cell will not fold correctly without the assistance of molecular chaperones. Chaperones have been defined as “a family of cellular proteins which mediate the correct folding of other polypeptides, and in some cases their assembly into oligomeric structures, but which are not components of the final functional structures” (75, 76). This definition implies that the predominant function of molecular chaperones is to transiently interact with other proteins, thereby preventing the formation of illegitimate interactions that might otherwise lead to deleterious protein aggregation. Chaperones generally seem to bind to exposed hydrophobic surfaces that will ultimately be buried in the folded state. Controlled release of a substrate protein from the chaperone, often driven by ATP hydrolysis, promotes folding into the native state. Repeated cycles of binding and release may be necessary for productive folding.
Enormous progress has been made in the elucidation of the major chaperones belonging to the Hsp60 (GroEL) and Hsp70 (DnaK) families. A wealth of information on the structural and functional properties of these chaperones has accumulated, and many excellent reviews on this topic are available (18, 40, 111, 196, 251, 257). However, our understanding of other chaperones is comparatively limited. Alternative chaperones are less abundant and less critical for protein folding than are DnaK and GroEL. However, since protein folding has been recognized as one of the central problems in biology, our knowledge about the contribution of minor chaperones to this process is catching up.
The purpose of this review is to draw attention to a family of low-molecular-mass chaperones, the α-crystallin-type proteins. The bulk of our knowledge about this chaperone class comes from studies of the name-giving lenticular α-crystallins. The two forms of α-crystallin,αA- and αB-crystallin, prevent protein precipitation and cataract formation in the vertebrate eye lens (33). Interestingly, α-crystallins not only are present in lenticular tissues but also have been found in many other tissues like heart, brain, and kidney (11). Because of the seminal finding of four α-crystallin-type proteins in Drosophila (133), it is well established that α-crystallins comprise a diverse protein family existing in most, but not all, animals, plants, bacteria, and archaea (43, 60, 192, 192a, 220, 349). The presence of α-crystallin-type Hsps in all kingdoms clearly points to important biological functions beyond their specialized role in clear vision. The discovery that α-crystallins can act as molecular chaperones (127, 138) boosted research on this class of stress proteins. The growing interest in this subject is reflected by a rapidly increasing amount of literature, which will be reviewed here.
Most information in this article will be presented from the perspective of a microbiologist. Whenever necessary and appropriate, complementary material on counterparts from higher organisms will be documented. More detailed information on eukaryotic α-crystallins can be found in other articles (11, 62, 71, 193, 268a, 349). The present review first introduces general principles of protein quality control in Escherichia coli and then gives details on the regulation, structure, and function of α-crystallin-type proteins. This information will finally be integrated into a model presenting how α-crystallins cooperate in the framework of a complex multichaperone network.
Normal Conditions
One of the most critical events in the biogenesis of a protein is the conversion of its linear amino acid sequence into the properly folded three-dimensional structure. As soon as a nascent polypeptide chain emerges from the ribosome, it is prone to misfolding and subsequent aggregation. Although many proteins may fold spontaneously, the initial folding of a significant portion of cellular proteins requires the assistance of molecular chaperones (39, 229). It has been estimated that 20 to 30% of all proteins in the prokaryotic cytoplasm transit through the DnaK or GroEL chaperone machineries before adopting their final conformation (77, 316) (Fig. (Fig.1A).1A). Chaperoning occurs both cotranslationally, while the polypeptide is being synthesized, and posttranslationally, after the complete amino acid chain has been released from the ribosome (39). Cotranslational folding requires DnaK and trigger factor, a ribosome-associated protein with peptidylprolyl-cis-trans isomerase and chaperone-like activities (66, 316). Both DnaK and GroEL contribute to posttranslational protein folding.
FIG. 1.
FIG. 1.
Simplified model of protein quality control under normal and heat shock conditions. (A) Under optimal growth conditions, the rate of transcription and translation is very high. As indicated by the thick arrow, most proteins fold spontaneously without (more ...)
An alternative fate for misfolded proteins is proteolytic degradation. About 20% of all synthesized polypeptides never reach their final destination because fatal errors have occurred during transcription or translation or because correct folding has not been accomplished (357). Before such detrimental proteins accumulate, they are removed by proteases (Fig. (Fig.1A).1A). Several universal ATP-dependent protease families have been described (96, 97). Interestingly, the analogy to the major chaperone classes extents beyond their common ATPase activity. Both chaperones and proteases are designed to recognize similar features that are found on unfolded proteins but not on native proteins, namely, surface-exposed hydrophobic patches. This related activity led to the evolution of a similar ring-like architecture of various chaperone and protease complexes (126, 357). Most intriguingly, the proteases involved in protein quality control have intrinsic chaperone activity, either within the same polypeptide (Lon, FtsH, and DegP) or located in associated components of a protease complex (ClpAP and ClpXP, where the ATP-dependent chaperone is underlined). The term “charonin” was invented for this type of multifunctional proteins or protein complexes (97, 272, 338). The tight combination of chaperone function with proteases suggests that the initial energy-dependent steps of the two processes are similar. Partial unfolding of substrate proteins is most probably the common prerequisite for both activities (304, 313, 351).
Protein synthesis in bacteria is much faster than in eukaryotes. As calculated from a synthesis rate of 15 to 20 amino acids per ribosome per s, E. coli produces some 30,000 polypeptides per min (39). This remarkable speed of translation requires a very efficient and accurate protein quality control system. Even if only 30% of the proteins need the attention of chaperones, almost 10,000 polypeptides per min are going through a chaperone cycle. Evidently, the decision of whether a polypeptide can be folded or must be degraded has to be made rapidly. Precise monitoring of the actual state of a protein is required to direct it to the appropriate pathway. It is not clear how the quality control system decides between (re)folding or breakdown when it faces a misfolded protein. Several tagging devices have evolved to sort out the hopeless cases that cannot be rescued by chaperones. Ubiquitinated polypeptides are removed by the proteasome in eucaryotes (47, 340). The N-end rule, variations of which apply to all known organisms, correlates the amino-terminal amino acid with the half-life of a protein (323, 339). Whereas certain residues confer a short-half life, others seem to stabilize a protein. The exposure of a destabilizing residue in damaged proteins directly routes them toward degradation, bypassing any refolding attempts. In E. coli, truncated polypeptides that result from abnormally terminated transcription are tagged by the SsrA system and thereby directed toward degradation (150, 329). A recent report demonstrates that abnormal proteins are susceptible to carbonylation, an unrepairable oxidative modification (70). This might provide the signal that a protein is irreparable and therefore destined for degradation. The associated chaperone components of the Clp proteases or the proteasome play a role in the decision whether a polypeptide can be salvaged (97, 357). Although important aspects of protein folding and degradation have been worked out over the last years, many details of the steps between the birth and death of a protein remain to be elucidated. The fate of every single protein in a cell constantly relies on a delicate balance between folding and degradation (121, 357). The rapid biogenesis of proteins in a growing cell puts a high pressure on the quality control machinery even under optimal conditions.
Stress Conditions
Once cellular proteins are folded, various stress conditions pose a serious threat to their integrity. Temperature variations, osmotic changes, antibiotics, solvents, or other chemicals not only interfere with transcription, translation, and protein folding but also often disrupt the faithfully acquired three-dimensional protein structure. The heat shock response elicited by a sudden increase in the ambient temperature is widely used as a model system for studying the impact of stress on biological systems. Proteins whose expression is induced on heat shock are generally called heat shock proteins (Hsps). It is not surprising that the classical chaperones and proteases are among them. All players involved in the regular protein quality control system described in the previous section are required to combat the damage inflicted by a thermal insult. On heat shock, a cell faces numerous problems. Transcription and translation slow because the RNA polymerase subunits RpoA, RpoB, and RpoD (σ70) are thermolabile (23, 211) and because the translation factor EF-G is susceptible to aggregation at elevated temperatures (211) (Fig. (Fig.1B).1B). Spontaneous folding of nascent polypeptides at high temperatures is error prone because interactive hydrophobic surfaces become exposed. Even subtle structural changes may suffice to inactivate cellular enzymes. It is evident that protein quality control under such circumstances becomes crucial for sustaining cellular metabolism and viability. In contrast to normal conditions, productive protein folding now occurs predominantly via the chaperone-mediated pathway due to a large number of thermolabile proteins (211). A large portion of already folded proteins gets partially or completely denatured and reenters the quality control system (Fig. (Fig.1B).1B). When the rate of denaturation outpaces the refolding capacity, increasing amounts of proteolysis-sensitive substrates are being generated.
The additional demand for folding support during acute stress is met by two strategies: (i) the level of preexisting quality control proteins is elevated; and (ii) additional chaperones that are not expressed or are only weakly expressed under nonstress conditions are induced to counteract severe damage. Members of the first class, which are abundant under all metabolic conditions, are DnaK and GroEL. α-Crystallin-type Hsps usually belong to the second class. Since these proteins are barely expressed at nonstress temperatures in most organisms, the induction factors after a temperature upshift can be very high (several hundred-fold [Table [Table1])1]) (258). Proteases are generally less abundant than chaperones regardless of the environmental conditions, indicating that protein refolding is preferred to proteolysis. Transcriptional induction after heat shock of most proteases was measured in the low to intermediate range (between 5- and 30-fold [Table [Table1])1]) (258). Although both chaperones and proteases are upregulated under stress conditions, many proteins seem to escape the quality control system and end up in aggregates. Polypeptides trapped in this state have long been considered dead-end products that cannot be rescued. Only recently, it was recognized that certain chaperones are able to solubilize aggregated proteins in vivo. The concerted action of Hsp104, Hsp70, and Hsp40 in yeast (92) or of ClpB and DnaK in E. coli (94, 211, 214, 347) recycles precipitated proteins into the folding pathway. Disaggregated material is released in a nonnative form that either can refold spontaneously or can be further processed by cellular chaperones.
TABLE 1.
TABLE 1.
Heat-inducible chaperone and charonin families in E. coli
In summary, nature has invented an arsenal of powerful strategies to maintain high-quality protein in the cell. Once a nascent polypeptide has folded correctly, it is not left alone. Problems arising within the life span of a protein are solved by chaperones and proteases, which assist in refolding or disposal of nonrefoldable molecules, respectively. The next section will look more closely at the different chaperone families that contribute to protein folding.
Traditionally, Hsps have been grouped into five major families. They were designated Hsp100, Hsp90, Hsp70, Hsp60, and small Hsps according to their molecular masses (37, 40, 213). Several members of the Hsp100 family are chaperone subunits of protease complexes. Hence, there is good reason to include the single-chain charonins, which bear both chaperone and protease functions in a single polypeptide, in the chaperone list. Hsp33, a novel chaperone whose activity is redox regulated, recently joined the club (140). The updated list of chaperone families therefore comprises seven members (Table (Table1).1). It should be noted, however, that more than 30 functionally uncharacterized heat shock genes and proteins have been identified by global transcriptome and proteome analyses in E. coli (46, 258, 330). Whatever their function might be, one may anticipate a growing number of chaperone families in the future.
Hsp70 (DnaK) and Hsp60 (GroEL)
The two major chaperone families are Hsp70 and Hsp60. They are also the by far best-characterized chaperones. DnaK and GroEL, the bacterial representatives of these classes, are among the most abundant cellular proteins, indicating their important role in protein folding. In the gram-negative and gram-positive model organisms E. coli and Bacillus subtilis, respectively, groEL is essential whereas dnaK is not (80, 183, 240, 271). In both species, serious growth defects and inviability of dnaK mutants were observed only at high temperatures (210, 240). In Streptomyces coelicolor A3(2), Pseudomonas syringae pv. glycinea, and Bradyrhizobium japonicum, all attempts to construct dnaK deletion strains failed suggesting that in some organisms the DnaK function might also be essential under physiological conditions (34, 151, 206). Multiple hsp70 or hsp60 genes have been identified in many organisms (83, 189, 273). Often, Hsp70 or Hsp60 homologs are not temperature controlled but are either constitutively expressed or induced by environmental cues other than heat. In some cases, family members seem to be able to functionally replace each other, e.g., the GroEL proteins of B. japonicum (84). Other seemingly similar proteins appear to have more specialized functions and are unable to restore the defect caused by a deleted family member, e.g., DnaK and HscA (Hsc66) of E. coli (123).
Both major chaperones recognize hydrophobic surfaces of unfolded proteins. To finish the folding job, they require specific cochaperones and ATP (Table (Table1).1). The DnaK cycle is driven by the concerted action of DnaJ and GrpE (18, 40). Briefly, DnaJ accelerates the ATPase activity and substrate binding of DnaK whereas GrpE functions as nucleotide exchange factor, promoting the exchange of ADP for ATP. Although details of the GroEL cycle are still disputed, it seems widely accepted that binding of ATP and GroES trigger conformational changes in the GroEL ring and promote folding of the polypeptide captured in its central cavity. Subsequent ATP hydrolysis discharges GroES and the substrate from the complex (40, 111, 126, 257). Among the many details that have been worked out for the Hsp70 and Hsp60 machines are the structural properties not only of the chaperone components but also of their cochaperones (85, 110, 131, 243, 360, 368). GroEL assembles into a cylindrical complex consisting of two homoheptameric rings with a large cylindrical chamber that accomodates substrate proteins (360). Unlike GroEL, DnaK acts as a monomer. There is no high-resolution structure of a full-length Hsp70 protein yet, but the crystal structures of the isolated ATPase and substrate-binding domains have been solved (85, 368). The latter contains a polypeptide-binding channel with a hydrophobic pocket. The completely different architectures of DnaK and GroEL are reflected by different substrate specificities. DnaK binds to short hydrophobic segments of nonnative proteins, whereas the GroEL ring encloses the entire substrate protein. Due to the size limitation of the central cavity, typical GroEL substrates are in the small to medium size range from 20 to 60 kDa (130). DnaK, on the other hand, is able to handle large proteins because it acts on surface-exposed hydrophobic peptide chains (211).
Hsp100
Although DnaK and GroEL are the main actors on the folding stage, there are many other chaperones adding to the fidelity of protein folding. These chaperones have more specialized functions and extend the limits of the DnaK- and GroEL-based folding machineries. With few exceptions to the rule, neither of the alternative chaperones is crucial for survival under physiological growth conditions. Hsp100 proteins are ATP-hydrolyzing chaperones that assemble into ring-shaped structures (100, 152, 369). All members of this family use ATP to promote changes in the folding and assembly of other proteins (269). The subsequent fate of a substrate protein depends on the actual Hsp100 member with which it is interacting (Table (Table1).1). ClpB directly binds protein aggregates. ATP-induced structural changes in ClpB are assumed to shear aggregates, preparing them for refolding by the DnaK system (94). ClpA and ClpX represent the substrate recognition subunits of the two-component ClpAP and ClpXP proteases (97, 313, 351). Although much smaller than the other family members, ClpX (46 kDa) is considered as Hsp100 relative. Unlike other family members, ClpX has only one instead of two ATP-binding sites. Polypeptides destined for proteolysis by ClpP are first bound and remodeled by the ATPase components ClpA or ClpX before they are translocated into the heptameric proteolytic ring (135, 254, 291). In the absence of the peptidase subunits, the ATPase oligomer acts as a bona fide chaperone, releasing the substrate in a folding-competent form (352, 356). For completeness, another type of two-component protease, ClpYQ (HslUV), also consisting of an ATPase subunit and a proteolytic component, should be mentioned (209, 260). Although inference from ClpA and ClpX suggests that ClpY (HslU) might possess chaperone activity, this has not been demonstrated yet. The invention of several two-component proteases implies that the intimate association of chaperones together with proteases improves the efficiency of protein degradation by promoting the unfolding of otherwise inaccessible substrate proteins. In fact, it has been shown that ClpP has no proteolytic activity when it is separated from ClpA (132).
Single-Chain Charonins
The same principle applies to single chain charonins, in which chaperone and protease activities are combined on a single polypeptide. It is not trivial to separate the two activities experimentally, but again it seems that chaperone activity might be a prerequisite for efficient proteolysis. Several lines of evidence strongly suggest that the membrane-anchored metalloprotease FtsH has chaperone activity. E. coli FtsH binds to denatured proteins and is involved in membrane protein assembly (4, 5). Moreover, growth retardation of an ftsH mutant can be partially suppressed by the overexpression of other chaperones (286). Chaperone-like activity has been demonstrated most explicitly for the FtsH yeast homolog Yme1, which directly binds to unfolded polypeptides and suppresses their aggregation (180). A very peculiar protein is the periplasmic serine protease DegP. It undergoes a temperature-dependent activity switch and functions as a chaperone at low temperatures and as a protease at elevated temperatures (303). Whether the activity of other charonins is regulated in a similar temperature-dependent manner remains to be tested. A proteolytically inactive variant of the Lon protease retains its substrate-binding capacity, congruent with a chaperone-like activity (337). Whether active refolding of bound substrates can be achieved is not clear. Direct chaperone activity involved in the assembly of membrane protein complexes has been suggested for the mitochondrial Lon protease (256). It should be pointed out again that the primary function of charonins is not to release substrate proteins for subsequent refolding. Although FtsH, DegP, and Lon, like ClpA and ClpX, sequester other proteins and thereby prevent inappropriate interactions leading to aggregation, the primary purpose of these chaperones is not to rescue other proteins but to prepare them for final destruction.
Hsp90
Three chaperone families remain to be discussed, Hsp90, Hsp33 and α-crystallin (Table (Table1).1). Of these proteins, only Hsp90 hydrolyzes ATP, and ATPase activity is essential for chaperone activity in vivo (241). ATP-independent chaperone-like activity can be demonstrated in vitro because Hsp90 bears two chaperone sites, one of which does not require ATP. Hsp90 is essential in yeast and Drosophila melanogaster but dispensable in E. coli and other bacteria (15, 36). In eukaryotes, Hsp90 is a dedicated chaperone involved in the folding of several signaling molecules including steroid hormone receptors (36, 137). The physiological function of HtpG, the bacterial Hsp90 protein, has not been discerned yet. In vitro, HtpG prevents aggregation of unfolded citrate synthase (CS) by transiently interacting with early unfolding intermediates (139). ATP hydrolysis is not necessary for this activity. A recent report indicates that HtpG has chaperone activity in vivo and is necessary for the optimal folding of certain cytoplasmic proteins in stressed E. coli cells (318).
Hsp33
E. coli Hsp33 is at present the only member of a novel redox-regulated chaperone class (140). Database searches suggested, however, that Hsp33 homologs are present in a wide variety of microorganisms. Hsp33 prevents the aggregation of thermally or oxidatively damaged proteins very efficiently in an ATP-independent manner (140). A feature that distinguishes Hsp33 from all other known chaperones is the reversible regulation of its chaperone activity by the redox potential of the cellular environment. Reduced Hsp33 is monomeric and inactive, whereas the oxidized chaperone is dimeric and functional (156a, 344a). The activity switch is brought about by the reversible disulfide bond formation between two pairs of cysteines that coordinate zinc in the reduced state (14). Zinc release and concomitant dimerization of Hsp33 induces structural rearrangements that lead to the formation of potential binding sites for unfolded proteins. Since it is thought that heat shock causes oxidative protein damage (21, 58, 197), it may not be surprising that a redox-sensitive chaperone is under heat shock control.
α-Heat Shock Proteins
The remaining tools in the protein-folding inventory that need to be discussed are the α-crystallin-type Hsps. The widely used nomenclature “small Hsps” for these chaperones is somewhat unfortunate because other Hsps, e.g., Hsp33, GroES, GrpE, and Hsp15 (a ribosome-associated Hsp [161]), are also small heat-inducible proteins but bear no resemblence to α-crystallin. To avoid any confusion, in the remainder of this review the more appropriate term “α-Hsp,” as suggested by de Jong et al. (61), will be used for the small Hsps that contain the characteristic α-crystallin domain.
As the (just discarded) designation “small Hsps” indicates, α-Hsps are low-molecular-mass proteins. Their size ranges from 12 to 43 kDa, with the majority being between 14 and 27 kDa. Although these proteins are small, their active entity usually is a large oligomer consisting of multiple subunits. The overall sequence homology between α-Hsps is much lower than in other chaperone classes. A common attribute of all α-Hsps is the presence of a conserved sequence of about 80 amino acids, which is generally referred to as the α-crystallin domain (43). This domain is preceded by an N-terminal region of variable length and considerable sequence diversity. In most cases, a short C-terminal tail extends downstream of the α-crystallin domain (Fig. (Fig.2).2).
FIG.2.
FIG.2.
FIG.2.
Amino acid alignment of bacterial and archaeal α-crystallins. Human αA- and αB-crystallins were added for comparison at the bottom. Abbreviations: Mjannas, M. jannaschii; Eco, E. coli; Vcholer, V. cholera; Ccr, C. crescentus; Mlo, (more ...)
During growth under optimal conditions, most bacteria produce either no or negligible amounts of α-Hsps. Under stress conditions, the induction factors both at the mRNA level and at the protein level can be dramatic (13, 115, 142, 178, 205, 220, 263, 276). Microarray-based expression profiling revealed that transcription of ibpA and ibpB, encoding the E. coli α-Hsp members, was heat induced by a factor of 300 (258). This was by far the highest increase among all heat shock genes (Table (Table1).1). IbpA and IbpB received their designation of “inclusion body-associated proteins” because they were initially characterized as E. coli proteins tightly associated with overexpressed recombinant proteins that had formed insoluble inclusion bodies (6). In general, α-Hsps seem to be dispensable. A temperature-sensitive growth defect of E. coli ibpAB mutants is barely detectable but becomes more pronounced in the additional absence of the dnaK gene (158, 319). Similarly, disruption of hsp30 in the fungus Neurospora crassa produces no clear phenotype at elevated temperatures but, the hsp30 mutant was extremely sensitive if heat stress was combined with carbohydrate limitation (248). Deletion of hsp16.6, the single α-Hsp gene in the cyanobacterium Synechocystis sp. strain PCC 6803, resulted in significantly decreased growth rates and in reduced photosynthetic activity on heat treatment (178). Probably the most drastic phenotype to date has been reported in mice, in which disruption of the eye lens αA-crystallin led to cataract formation due to rapid inclusion body formation (33).
While most chaperones consume energy, α-Hsps are generally believed to be ATP-independent chaperones (138). As a consequence, they lack the refolding capacity of the major chaperones because unfolding and release of folding intermediates cannot be triggered. Nevertheless, α-Hsps have been added to the catalogue of molecular chaperones because they bind to denatured proteins and thereby suppress inappropriate interactions leading to the precipitation of aggregates. The action of α-Hsps maintains substrate proteins in a folding-competent state (72, 175). The reservoir of substrate proteins associated with α-Hsps remains amenable to subsequent refolding by the major chaperone machineries (341). It is important to consider that α-Hsps alone will not efficiently “mediate the correct folding of other polypeptides,” according to the chaperone definition given above (75, 76). Only in the context of a multichaperone network are they able to enhance protein folding.
α-Crystallins are widely distributed among all kingdoms, and their existence has been reported in numerous organisms from bacteria to humans. It is noteworthy, however, that not all organisms contain α-Hsps. Owing to the steadily growing number of whole-genome sequences, it is now possible to determine the exact number of α-Hsp genes in a diverse array of organisms. Table Table22 illustrates that this number can vary substantially. With the exception of Halobacterium sp. strain NRC-1, whose genome encodes five putative α-Hsps, all other archaea investigated so far have genomes that encode either one or two. The mere presence of these proteins in thermophilic archaea seems puzzling since many of them are devoid of DnaK, DnaJ, and GrpE homologs (192), which are generally believed to be more important for protein folding than are α-Hsps. The universal occurrence of α-crystallins in the archaeal kingdom might be indicative of an early phylogenetic origin of this protein family. Perhaps they were established before the more efficient DnaK machinery was invented. In fact, it has been proposed that archaea that contain dnaK, dnaJ, and grpE genes acquired them from bacterial donors by lateral gene transfer (99).
TABLE 2.
TABLE 2.
Number of α-crystallins in archaea and bacteria
Not only thermophilic archaea but also the bacterial thermophiles Thermotoga maritima and Synechococcus vulcanus each contain a single α-Hsp (Table (Table2).2). The S. vulcanus protein HspA accumulates after heat treatment (263). Apart from global genome and proteome analyses, detailed information about the heat shock response in thermophilic organisms is scarce. Representative thermophiles from all three phylogenetic domains are capable of mounting a heat shock response (327). It appears that organisms adapted to permanent growth at ferocious temperatures between 60 and 100°C still require responsiveness to temperatures beyond their optimal growth range.
The complete absence of α-crystallin genes in a number of bacteria became evident during mining of genome-sequencing data (Table (Table2).2). What do the microorganisms lacking α-Hsps have in common? First, they have rather small genomes, ranging from 0.58 to 2.27 Mb. The 0.58-Mb genome of Mycoplasma genitalium demonstrated that the minimal gene set of self-replicating organisms comprises some 470 coding regions (88). As one might predict, a streamlined genome like this devotes only few resources to superfluous functions such as regulation, DNA repair, and protein quality control. The minimal Hsp set consists of GroEL and GroES, DnaK, DnaJ and GrpE, ClpB, Lon, and FtsH. Both Mycoplasma species sequenced lack genes coding for ClpA, ClpP, ClpX, HtpG, DegP, and α-Hsps (88, 124). Treponema pallidum and Helicobacter pylori, with genomes approximately twice and three times the size of the M. genitalium genome, respectively, contain the classical set of Hsps listed in Table Table11 with the exception of α-Hsps (89, 324). Since α-Hsps are unable to productively refold denatured proteins, they are probably the chaperones of choice for omission by a cell with a limited genome. In line with the assumption that small genomes go along with the absence of α-Hsps is the presence of multiple α-Hsps in organisms with relatively large genomes such as B. subtilis, rhizobia, and eukaryotes (Table (Table2).2). The larger the genome, the more genes seem to be devoted to the adaptation to atypical conditions. It should be pointed out, however, that a small genome does not strictly coincide with the absence of α-Hsps. Buchnera sp. strain APS (0.64 Mb) and Rickettsia prowazekii (1.1 Mb) each carry an α-crystallin-type protein (Table (Table2).2). Deducing the absence of these proteins from the limited genome size of these two species would have been misleading.
Why are α-Hsp genes present in some organisms but absent in others? Probably more important than the genome size is the life-style of a bacterium and the ambient temperature it usually faces. Buchnera species are obligate endosymbionts of aphids. Their limited gene reservoir renders them completely dependent on a mutualistic relationship with the insect (285). Rickettsia species, the living relatives of mitochondria, also are intracellular parasites. Although their life-style resembles that of Chlamydia species, rickettsias are normally found in arthropods such as lice and ticks. Only occasionally do they infect humans and cause serious diseases (7). The preference for insects, whose body temperature fluctuates with the ambient temperature, might explain why Rickettsia and Buchnera species carry an α-Hsp gene in their limited gene set. Most strikingly, all presently known microorganisms without any α-Hsps are parasites and/or pathogens of human and animals. Some of them are degenerated to such an extent that they have become obligate intracellular human parasites, e.g., the Chlamydia species (252). In their more or less isothermal niche, the mammalian host, an elaborate system responding to temperature fluctuations might become obsolete. Incidentally, the absence of α-Hsps goes along with the absence of cold shock proteins (CSPs) in most cases. The only exception, Haemophilus influenzae, encodes just a single CSP, whereas α-Hsp-containing organisms, such as E. coli, B. subtilis, and Lactobacillus lactis, generally produce multiple CSPs during cold stress (98, 361). CSPs function as RNA chaperones, facilitating the translation of mRNA that tends to form secondary structures after a temperature downshift. Assuming that the simultaneous lack of α-Hsps and CSPs is no coincidence, it seems as if living inside mammalian hosts poses few thermal challenges and therefore obliterates the need for sophisticated temperature-responsive systems.
B. subtilis, Halobacterium sp. strain NRC-1, and rhizobial species are exceptional among bacteria and archaea in that they encode more than two α-Hsps (Table (Table2).2). Of the three putative α-crystallin-type proteins of B. subtilis, only YocM and CotM were recognized as family members during the initial open reading frame annotation (167). Like many potential α-crystallins in other annotated genome sequences, B. subtilis YdfT was categorized as a protein with unknown function. In fact, the similarity of CotM, YocM, and YdfT to other α-crystallins is low (Fig. (Fig.2).2). CotM is a dedicated α-crystallin involved in the assembly of the outer spore coat (120). Evidence for a chaperone-like activity of CotM was not found. CotM, YdfT, and YocM all might have rather specialized functions that do not require all conserved α-crystallin residues.
Multiple α-Hsps were detected during proteome analysis of various plant root-nodulating bacteria (205, 220, 226). A more detailed investigation of B. japonicum extracts uncovered at least 10 heat-induced small proteins belonging to the α-crystallin family (219). On the basis of their primary amino acid sequence, the α-Hsps were tentatively divided into two classes, class A and class B (220). Class A proteins (HspA, HspB, HspD, HspE, and HspH) are closely related to the E. coli IbpA and IbpB proteins (Fig. (Fig.2).2). Class B α-Hsps (HspC and HspF) are distinguished from class A proteins by their much longer N-terminal region and a shorter C-terminal extension. They have little similarity to E. coli α-Hsps. The presence of two α-Hsp classes was also found in Bradyrhizobium sp. (Parasponia) and in Rhizobium sp. strain NGR234 (235). Additional evidence for the presence of multiple α-Hsps and for the existence of distinct classes in rhizobia was provided by the determination of the entire genome sequence of Mesorhizobium loti and Sinorhizobium meliloti (89, 143). Eight α-Hsp genes encoding four class A and four class B proteins were identified in the first organism, and five genes encoding three class A and two class B proteins were identified in the latter. In this respect, the situation in rhizobial cells is similar to that in plant cytosol, in which three classes of α-Hsps (class I, II, and III) have been described (268a, 349).
α-Hsps are not the only rhizobial chaperones that are present in multiple copies. Several groESL operons or groEL genes were found not only in Rhizobium leguminosarum, S. meliloti, B. japonicum, and M. loti but also in many other microorganisms (83, 105, 144, 238, 345). What could be the underlying rationale for the evolution of such multigene families? At least four different reasons can be envisaged. (i) Simultaneous induction of redundant copies of a stress gene rapidly elevates the cellular pool of that protective protein class. Such a coordinated parallel induction of α-Hsps was observed in B. japonicum (220). (ii) Providing individual family members with different promoter sequences permits induction in response to a variety of stimuli, a strategy used in the case of rhizobial groESL operons (12, 83). (iii) A multigene family relieves the individual genes from functional constraints. Therefore, each gene is free to evolve, allowing it to acquire new functions. The B. subtilis CotM protein, for example, might be the product of such mutational diversification resulting in its role in sporulation. (iv) Given that a protein functions as an oligomer (as GroEL and α-Hsps do), slightly different versions of that protein might assemble into hetero-oligomers. Mixed oligomers probably possess substrate specificities or functions slightly different from homo-oligomeric complexes (312). Whatever the exact reason for a gene family might be, it is easily conceivable that iterated stress genes allow a more flexible response to changing conditions than a single gene.
Eukaryotes are well known for containing multiple α-crystallins. Saccharomyces cerevisiae inhabits the lower end of the scale with two α-Hsps (Hsp26 and Hsp42) (93), whereas plants lie at the upper end. The Arabidopsis thaliana genome exodes 19 α-Hsps. Six families of plant α-Hsps can be distinguished based on their sequence similarities and their cellular localization. Three families (I, II, and III) reside in the cytosol; one is localized to the chloroplasts, one is localized to the mitochondria, and one is localized to the endoplasmic reticulum (268a, 348, 349). Nine human α-Hsps, including αA- and αB-crystallin, have been described (144). Once thought to be eye lens-specific proteins, mammalian α-crystallins have now been found in many cell types (11, 193). In contrast to plant α-Hsps, the mammalian family members seem to be restricted to the cytosol and to the nucleus and do not localize to other cellular compartments.
Members of the α-Hsp superfamily consist of three regions, a characteristic α-crystallin domain flanked by a poorly conserved N-terminal region and a short C-terminal extension (43, 61). Extensive alignments and phylogenetic analyses of plant and animal α-Hsps can be found elsewhere (43, 61, 268a, 348-350). An overall alignment of 65 α-Hsps from archaea and bacteria reveals only very few highly conserved positions (Fig. (Fig.2).2). The prototype α-crystallins, humanαA- and αB-crystallin, are listed for comparison. The sequence comparison clearly demonstrates that α-Hsps are related but quite distinct. Pairwise alignments between Methanococcus jannaschii Hsp16.5, E. coli IbpA, or B. subtilis CotM and human αA-crystallin show that the sequence identity is as low as 23, 21, and 19%, respectively. Closely related proteins like E. coli IbpA and IbpB or human αA- and αB-crystallins have not more than 52 or 58% identical amino acids. Rhizobial α-Hsps show the highest degree of sequence similarity, provided that they belong to the same class. For example, 74% the amino acids in B. japonicum HspA and HspB (class A) and 61% of those in HspC and HspF (class B) are identical.
As can be seen in Fig. Fig.2,2, not a single amino acid is entirely conserved throughout all the proteins examined. Only five residues (corresponding to G62, L111, A122, G127, and L129 of M. jannaschii Hsp16.5) are present in more than 80% of all sequences. The last three residues occur in an A-x-x-x-n-G-v-L consensus motif toward the end of the α-crystallin domain; this motif is the most significant indicator of the domain (43, 61, 349). Almost universally conserved are the G127 and L129 residues, which occur in all but one protein. In CotM from B. subtilis, the residue equivalent to G127 is a glutamine. In addition, CotM carries replacements of other conserved residues (e.g., the amino acids equivalent to P61 and G62 in Hsp16.5 are lysine and histidine in CotM). Probably owing to this diversification, CotM has no discernible chaperone activity and serves a unique function in spore coat formation (120). Hsp1 from Halobacterium sp. strain NRC-1 contains a cysteine instead of the conserved leucine at position 129. As for most of the sequences listed in Table Table2,2, nothing is known about the functional role of this putative protein. It is possible that Hsp1, like CotM, has structural and functional properties different from standard α-Hsps.
All five highly conserved amino acids reside in the α-crystallin domain, which carries a few additional moderately conserved residues. The flanking regions are even more divergent. Large deviations in sequence and length are evident in Fig. Fig.2.2. An alignment can be enforced only at the expense of numerous gaps, in particular in the N-terminal region. Very few residues are retained in more than 40% of all sequences. The only exceptions are two characteristic isoleucines (I144 and I146 in Hsp16.5) in the C-terminal extension. They are separated by a single variant amino acid and play an important structural and functional role, at least in M. jannaschii Hsp16.5, wheat Hsp16.9, and both classes of B. japonicum α-Hsps (see below) 155, 338a; S. Studer, M. Obrist, N. Lentze, and F. Narberhaus, submitted for publication).
As indicated in the quality control section (see above), it is important that the cellular level of chaperones and proteases be adjusted to the prevailing environmental conditions. The cellular level of chaperones and proteases must be strictly controlled because both excessive and limited amounts compromise the fitness of a cell. The regulatory mechanisms controlling their expression are very diverse. Regulation in most cells occurs at the level of transcription. In eukaryotes, elevated expression of heat shock genes is accomplished by transcriptional activation. With some modifications to the theme, the general principle is conserved in yeast, vertebrates, and plants. In brief, an inert non-DNA-binding heat shock transcription factor (HSF) is converted upon heat shock to a transcription-competent activator that binds to a cis-acting heat shock element (HSE) in the promoter region of heat shock genes (212, 236). The activation process of the HSF goes along with its trimerization and phosphorylation. Stress-induced molecular chaperones, most importantly Hsp70, autoregulate the heat shock response by direct binding to the activation domain of HSF (212, 284).
Heat shock regulation in archaea is largely unsolved. The archaeal proteins involved in basal transcription are related to those of the eukaryotic transcription machinery (19, 179, 300). However, archaea have neither an identifiable HSF nor an HSE in heat shock gene promoter regions (192). Bacterial heat shock promoters or regulatory elements are also absent in archaeal genomes. Transcription of the heat-inducible cct1 (chaperonin-containing Tcp-1) gene in the archaebacterium Haloferax volcanii requires only sequences within the core promoter region (320). The finding of multiple variants of the promoter-binding TATA-binding protein led to the hypothesis that alternative forms of TATA-binding protein are responsible for transcription under heat shock conditions (321).
The latter strategy is strikingly reminiscent of heat shock regulation in E. coli. It uses alternative transcription factors, so-called sigma factors, to modulate heat shock gene expression. Bacterial sigma factors are subunits of the RNA polymerase that confer promoter specificity to the core enzyme (103, 134, 358). Specific transcription of the majority of heat shock genes in E. coli depends on the sigma factor σ32 (RpoH) (102). The cellular concentration of σ32 increases transiently after a temperature upshift, primarily as the result of elevated translation of rpoH mRNA and of increased stability of the sigma factor. At normal temperatures, σ32 is rapidly degraded by FtsH. The requirement of DnaKJ for σ32 proteolysis couples the availability of chaperones to heat shock gene transcription and provides a homeostatic heat shock control mechanism (38, 102, 366). The ibpAB operon, which encodes both α-Hsps of E. coli, belongs to the σ32 regulon (6, 46) (Fig. (Fig.3A).3A). Immunodetectable levels of IbpA and IbpB proteins in rpoH mutants suggest, however, that a σ32-independent pathway participates in the expression of these chaperones (6, 170). Recently, it was found that ibpB alone can be transcribed from a σ54 (RpoN)-dependent promoter (164a).
FIG. 3.
FIG. 3.
Regulation of bacterial α-Hsp genes. A representative organisms for each regulatory strategy is listed. The regulated genes and corresponding regulators are indicated. Promoters are presented as −10 and −35 regions. Known repressor-binding (more ...)
Regulation by alternative sigma factors has also been described for two other bacterial α-Hsp genes (Fig. (Fig.3A).3A). Legionella pneumophila gspA is transcribed from a σ70-type and a σ32-type promoter (2, 3). Induction of gspA expression by stress stimuli and during intracellular infection occurs predominantly via the latter promoter. Hsp16.3 of Mycobacterium tuberculosis is, at least in part, dependent on SigF, one of many stress-responsive sigma factors in this organism (194). Hsp16.3 (Acr) is not heat shock responsive but accumulates in the transition to stationary phase, during hypoxia and infection of macrophages (364, 365). Many conditions that enhance the SigF level have no effect on hsp16.3 expression, indicating that SigF is not the sole regulator of this gene. The involvement of the two-component regulatory pair Rv3133c/Rv3132c has recently been inferred from a microarray approach (283).
During investigation of other heat shock regimes, it turned out that positive control by alternative sigma factors is not typical of many other bacteria. Rather, transcriptional repression of heat shock genes is a widespread strategy found in many phylogenetically distinct bacteria. Overlapping or nearby repressor and RNA polymerase-binding sites prevent transcriptional initiation under circumstances where the repressor is competent for DNA binding. A number of heat shock gene repressors have been identified recently (114, 222). Some of them also control α-Hsp genes (Fig. (Fig.3B).3B). An intriguingly simple mechanism was discovered in Streptomyces albus. At low temperatures, RheA (for “repressor of hsp eighteen”; formerly OrfY) inhibits the transcription of hsp18 (276, 277). As the result of a thermally induced conformational change, the repressor is unable to interact with its target sequence (an inverted repeat) at elevated temperatures (274). The transition between the active and inactive forms is fully reversible. RheA thus acts as a cellular thermosensor, directly correlating heat shock gene expression to the ambient temperature.
hsp18 of Clostridium acetobutylicum, hsp18 of Leuconostoc oenos (Oenococcus oeni), and hsp16.4 of Streptococcus thermophilus are preceded by putative CtsR target sites (64). CtsR (for class three stress gene repressor) was initially identified in B. subtilis as negative regulator of the clpC operon (64, 163). It blocks transcription of target genes at normal temperatures through binding to a conserved heptanucleotide repeat (Fig. (Fig.3B).3B). CtsR is specifically degraded by the ClpCP protease during stress. Since expression of the Clp components (and some additional regulatory factors) is under CtsR control, proteolysis of the repressor constitutes a built-in autoregulatory loop (65, 164). Putative ctsR homologs and potential CtsR-binding sites upstream of heat shock genes were documented in a number of gram-positive microbes (64). Temperature-regulated transcription from housekeeping promoters was demonstrated for the C. acetobutylicum and O. oeni hsp18 genes (142, 267). However, experimental proof that CtsR mediates heat shock control of α-Hsp genes in these and other gram-positive bacteria remains to be generated.
Neither of the three α-crystallins of B. subtilis is temperature regulated. CotM is induced at late stages during sporulation and maintains the structural integrity of the outer spore coat (120). Both an alternative sigma factor (the late sporulation sigma factor σK) and a repressor protein (GerE) contribute to its proper temporal and spatial expression (Fig. (Fig.3C).3C). Similar dual control of ydfT led to its alternative designation, cotP (255). Although expression of CotM and CotP is restricted to sporulation, they seem to be dispensable for this process.
A number of bacterial α-Hsp genes and operons are regulated by mechanisms that cannot be assigned to either transcriptional activation or repression. Long untranslated regions (5′UTRs) were found upstream of various rhizobial α-Hsp genes and upstream of hspA of Synechococcus vulcanus (223, 224, 235, 263) (Fig. (Fig.3D).3D). Temperature-regulated transcription of all these genes was initiated at vegetative promoters. A novel regulatory mechanism controlling mRNA stability in a temperature-dependent fashion was inferred from the fact that the hspA transcript of S. vulcanus is more stable at 63 than 50°C. Unknown factors might be involved in this process (263). The 5′UTR of at least 15 small heat shock operons from B. japonicum, Bradyrhizobium sp. (Parasponia), Rhizobium sp. strain NGR234, and Mesorhizobium loti was designated ROSE, acknowledging its role in repression of heat shock gene expression (223, 235). Although a repressor-type mechanism was favored initially, there now is accumulating evidence that ROSE acts at the posttranscriptional level. RNA structure predictions suggest that the highly conserved 3′ region of all known ROSE sequences folds into a stem-loop structure that masks the ribosome-binding site (RBS) (234). A detailed mutagenesis study on a representative ROSE element demonstrated that the exchange of individual nucleotides potentially involved in base pairing relieves α-Hsp gene repression at low temperatures. The current model holds that mRNA folding at low temperatures has two consequences. It blocks access of ribosomes to the RBS and thereby impairs translation. The presumed secondary structure probably also promotes RNase cleavage and rapid decay of ROSE-containing mRNAs, explaining the minute amounts of α-Hsp transcripts at low temperatures. According to this model, high temperatures would melt the hairpin structure, allowing ribosomes to access the RBS. Ribosome entry then would initiate translation and simultaneously protect ROSE-containing mRNA from degradation.
A noteworthy feature of several α-Hsp genes is their extrachromosomal location. Small plasmids carry the low-molecular-mass stress proteins of Streptococcus thermophilus (239, 298, 299). On plasmids pER16 (4.5 kb), pER35 (10 kb), pER36 (3.7 kb), and pER341 (2.8 kb) originating from different S. thermophilus strains, the only other open reading frame encodes a rolling-circle replication protein (298, 299). The 6.5-kb plasmid pCI65st from S. thermophilus NDI-6 codes for two almost identical α-Hsps (Hsp1 and Hsp2; an alignment is given in Fig. Fig.2),2), a replication protein, a putative enolase, and HsdS, a putative type 1 restriction modification enzyme (239). These streptococcal replicons are readily lost at low temperatures but stably maintained at optimal growth temperatures of 42°C (239, 298). The plasmid stability suggests that the α-Hsps are beneficial to lactic acid bacteria during fermentation of dairy products.
Sequencing of rhizobial genomes revealed that some of their multiple α-Hsp genes are also located on extrachromosomal replicons. M. loti contains the megaplasmids pMLa (352 kb) and pMLb (208 kb). The latter bears the locus mll9627, coding for one of eight α-crystallins (143, 235). In Sinorhizobium meliloti, three of five α-Hsps are encoded on symbiotic megaplasmids. The locus SMa1118 lies on pSymA (1.4 Mb), and SMb21294 and SMb21295 are on pSymB (1.7 Mb) (89). The presence of several α-Hsps in bacteroids suggests that these proteins play a role in establishing a successful plant-microbe interaction (226). A plasmid-borne α-crystallin gene was also found in Buchnera aphidicola, the endosymbiont of aphids (334). Other genes harbored by this 8.5-kb plasmid are involved in leucine biosynthesis. A remarkably similar clustering of an ibpB-like gene with leucine biosynthetic genes was observed on the chromosome of Azotobacter vinelandii (195). Whether the close association of α-Hsp genes with amino acid metabolism genes is a coincidence or functionally relevant is unclear.
Homo-Oligomeric Complexes
A hallmark of α-Hsps is their tendency to “socialize,” or in other words, to assemble into large oligomeric complexes. There is ample evidence that oligomerization is a structural prerequisite for chaperone activity of the vast majority of α-Hsps. Neither naturally occurring multimerization-incompetent α-crystallins nor mutated variants that have lost the ability to form large complexes are efficient chaperones 160, 181, 182, 331; Studer et al., submitted). In many cases in which bacterial α-Hsps have been studied biochemically, they were reported to build complexes consisting of approximately 24 subunits (156, 204, 262, 310). Formal proof for such an organization stems from the crystal structure of the M. jannaschii Hsp16.5. A total of 24 monomers form a spherical complex with 14 open windows (155) (see Fig. Fig.5).5). Electron microscopy (EM) images also revealed similar spherical complexes for human αB-crystallin, human Hsp27, native bovine α-crystallin, and yeast Hsp26 (107, 112).
FIG. 5.
FIG. 5.
Overall structure and subunit interactions of Methanococcus jannaschii Hsp16.5. (A) In the space-filling model of the hollow sphere, each tetramer is represented in one color with different shadings. At the bottom, the interior of the sphere is viewed (more ...)
Examples of both smaller and larger assemblies than 24-mers have been documented. M. tuberculosis Hsp16.3 forms a triangular structure comprising a nonamer composed of a trimer of trimers (44). Pea Hsp18.1 and Hsp17.7, two representatives of cytosolic plant α-Hsps, produce discretely sized complexes containing 12 identical subunits (174). Murine Hsp25 exists predominantly as a hexadecamer (72, 74). At the opposite extreme of the oligomeric scale are the proteins that form large and heterogenous assemblies. α-Crystallin from vertebrate eye lenses is normally isolated as an 800-kDa complex comprising 32 subunits. However, various other assemblies from 280 kDa to 10 MDa have been reported (101). The majority of E. coli IbpB is eluted from gel filtration columns as globular structures exceeding 2 MDa (282, 341). Electron micrographs reveal pronounced size heterogeneity from small roughly spherical complexes with a diameter of 15 nm (approximately 600 kDa) to 100-200-nm structures that interact over time to form loose aggregates of micrometer size (282).
Regardless of the subunit composition, all those diverse assemblies described above efficiently protect other proteins from aggregation, illustrating that a composition of 24 subunits is not a structural prerequisite for chaperone activity. The astounding diversity of α-Hsp assemblies also is the reason why the minimal oligomeric requirement for chaperone activity is not clear-cut. The monomeric Hsp12.6 from Caenorhabditis elegans is unable to prevent the aggregation of test substrates (181). Hsp12.2 and Hsp12.3, two other exceptionally small members of the α-crystallin family of C. elegans, assemble into tetramers that are devoid of any chaperone activity (160). In contrast, Hsp20 from rats tends to form dimers that act as poor chaperones (331). A truncated version of human αB-crystallin (αB57-157) that contains only the isolated α-crystallin domain builds dimers with significant chaperone activity (81). Unlike other α-Hsps, yeast Hsp26 requires temperature-assisted dissociation of a 24-mer into dimeric species in order to become an efficient chaperone (112). Tetramers of murine Hsp25 that occur as intermediates in the assembly of 16-mers have been shown to bind troponin T, a structurally labile marker protein for myocardial cell damage (73). This short list of observations already implies that the correlation between the oligomeric status and chaperone activity is different for individual α-Hsps.
Hetero-Oligomeric Complexes
The tendency of α-Hsps to generate higher-level structures poses the question whether oligomers always contain identical subunits or whether mixed oligomers can be formed (provided that different α-Hsps occur in the same cell or cellular compartment). Native α-crystallin isolated from the eye lens is composed of the closely related subunits αA- and αB-crystallins in a 3:1 stoichiometry (129). Under in vitro conditions, however, any ratio can be formed (333). Several reports demonstrate that αA- and αB-crystallins are able to interact with other members of the α-crystallin family. αB-crystallin copurifies with human Hsp28 or with rat Hsp27 (146, 367). On mixing of purified components in one study, heteropolymers from any combination of bovine αA-crystallin, αB-crystallin, and mouse Hsp25 could be detected (202). An interaction between Hsp27 and αB-crystallin was demonstrated by the yeast two-hybrid system (27, 190). Finally, fluorescence-labeled αA-crystallin readily exchanged with αB-crystallin and with Hsp27 (31). All these findings strongly suggest that hetero-oligomerization is a common phenomenon in mammalian cells.
The formation of mixed α-Hsp complexes in plants and bacteria appears to be more restricted than in mammals. Most of the multiple α-Hsps that are being produced in plants are prevented from interacting with each other because they are housed in different cellular compartments (349). However, three distinct classes occur in the cytoplasm. The recombinant pea proteins Hsp18.1 and Hsp17.7 (representative class I and class II members, respectively) were analyzed for complex formation in vitro (119). Both proteins strictly assembled into homo-oligomeric complexes and did not form hetero-oligomers. EM revealed differences in the shapes of Hsp18.1 and Hsp17.7 complexes, which might prevent the exchange of subunits between α-Hsps from different classes (174). Isolated wheat Hsp16.9 and pea Hsp18.1, two class I proteins, readily exchanged subunits (338a). The finding that isolated native class I oligomers from soybean, rice, mung bean, and pea consist of at least 8 to 15 different isoforms also suggests that α-Hsps of the same class produce hetero-oligomeric complexes in vivo (141).
Separate formation of dodecameric complexes was also described for class I and class II proteins from tobacco protoplasts (157). Interestingly, class I- and class II-specific homo-oligomers coassembled into heat shock granules (HSGs), large cytosolic complexes that appear under stress conditions and disassemble during recovery (237). Their inner core is probably composed of α-Hsps, whereas Hsp70 and Hsp40 seem to be associated with the surface of the granules (296). Denatured proteins, mRNA, RNA-binding proteins, and heat shock transcription factors might also be enclosed in HSGs (149, 237, 268). The integration of α-Hsps into HSGs is not the result of non-specific aggregation but an ordered assembly process (157). Only class II complexes can jointly build the core of a HSG, whereas class I proteins cannot. Remarkably, preexisting class II supercomplexes can then recruit class I homo-oligomers. This assembly process is highly specific because plant α-Hsps from other classes are not incorporated into HSGs.
Copurification studies with bacterial α-Hsps provided direct evidence for complex formation between two members of the same class (310). Isolated hetero-oligomers displayed chaperone activity indistinguishable from either homo-oligomeric complex. Mixed oligomers were also obtained with class A proteins from different organisms, e.g., E. coli IbpB and B. japonicum HspB. However, they were never observed between members of two different classes, e.g., E. coli IbpB and B. japonicum HspC or B. japonicum HspB and HspC, suggesting a structural barrier for oligomerization of distantly related α-crystallins.
Is the formation of mixed oligomers the result of a fortuitous interaction of structurally related proteins, or might it be of functional significance? In principle, the multimerization of similar but not identical subunits offers the opportunity to take advantage of slightly different properties of the individual particles. Most likely, the differences between certain compositions are subtle and are detectable only by rigorous biochemical investigation. Advances in this direction have centered on the lenticular α-crystallins. Recombinant αB-crystallin was shown to be a better chaperone than αA-crystallin, in particular at physiological temperatures (57, 311). Optimal chaperone activity probably is sacrificed for stability reasons in the naturally occurring 3:1 stoichiometry of αA- and αB-crystallins. The mixed complex has greater thermal stability and is more compact than is either homo-oligomer (312). A stable and long-lived structure might be the ideal solution in the eye lens since there is no protein turnover in this tissue.
Apart from structural considerations, it is conceivable that variations in the subunit composition might alter the substrate specificity of α-crystallins. Little is known about substrate selection of these chaperones. If different α-crystallins were to recognize specific target sites in unfolded proteins, the coassembly of different subunits should influence the binding properties. It is plausible that the rearrangement of α-crystallin complexes provides a means of tailoring the quatenary structure and functional properties of α-crystallins according to the actual needs.
Plasticity of Oligomer Formation
The formation of heteromeric structures suggests that α-Hsp assemblies are dynamic and are shaped by the frequent exchange of subunits. In fact, EM examination of various family members revealed highly variable quaternary structures (74, 107, 108, 112, 186, 282). Processed cryo-EM images uncovered a high degree of plasticity in the quaternary structure. Human αB-crystallin particles ranged in diameter from 80 to 180 Å, native bovine lens α-crystallin (3:1 molar ratio of αA- and αB-crystallins) ranged from 120 to 200 Å, and human Hsp27 ranged from 90 to 220 Å (107, 108). Unlike other family members, Methanococcus jannaschii Hsp16.5 was monodisperse and formed a rigid structure of rather homogenous size between 110 and 130 Å (107, 156). Apparently, this precisely defined particle was a proper choice for crystallization and structure determination (155). Despite a wide range in particle diameter and subunit composition, most α-Hsps imaged so far seem to fashion spherical assemblies with a central cavity, similar to the Hsp16.5 complex. It is as if football-like structures can be achieved with different numbers of subunits.
In an ordered assembly pathway, smaller particles serve as building blocks for multimeric complexes. Three trimers, for instance, produce the triangular nine-subunit complex of Mycobacteriumtuberculosis Hsp16.3 (44) (Fig. (Fig.4A).4A). Dimers have been postulated as building blocks of the dodecameric Hsp16.5 particle of Methanococcus jannaschii (155) (Fig. (Fig.4B).4B). Intermediates of the assembly pathway were not revealed by size exclusion chromatography since Hsp16.5 eluted as a single sharp peak representing a 24mer (156). In other instances, α-Hsp complexes are in a highly dynamic equilibrium with smaller and larger particles. The hexadecameric murine Hsp25 is in a concentration-dependent equilibrium with tetramers and dimers, indicating that both particles occur during the assembly pathway (74) (Fig. (Fig.4C).4C). Elevated temperatures induced the cooperative association of hexadecamers to large granules, which exist in slow equilibrium with the smaller particles. Quite remarkably, tetramers, hexadecamers, and granules of Hsp25 acted as chaperones in suppressing protein aggregation. A completely different pathway was postulated for Hsp26 from Saccharomyces cerevisiae (112). This protein is an efficient chaperone only at elevated temperatures. Heat shock temperatures trigger the dissociation of a 24-mer of Hsp26. The resulting dimers recognize and bind substrate proteins before they reassemble into large chaperone-substrate complexes clearly exceeding the original complexes (Fig. (Fig.4D).4D). It was concluded that yeast Hsp26 is a temperature-regulated chaperone whose activation is achieved by dissociation of a 24-mer that can be regarded as inactive storage form of the chaperone.
FIG. 4.
FIG. 4.
Postulated assembly pathways of α-Hsp complexes. Particles competent for binding unfolded proteins are shaded in gray. ΔT indicates a temperature upshift. For further details, see the text.
Comparative size exclusion chromatography of Hsp26 and bovine α-crystallin showed that the thermoresponsiveness found for Hsp26 is not a mechanism common to all α-Hsps. The α-crystallin complex did not disassemble during heat treatment (112). It is evident that the α-crystallin-type proteins that are induced in response to stimuli other than heat stress must act differently from Hsp26. Many α-Hsps function as efficient chaperones not only on thermally but also on chemically denatured substrates at low temperatures in vitro (e.g., on dithiothreitol [DTT]-treated insulin) (1, 188, 253). While temperature-mediated dissociation of α-Hsps might not be a universal phenomenon, more subtle temperature effects on the structural properties, chaperone activity, and subunit exchange of various family members are common. Of all parameters examined (temperature, ionic strength, pH, and Ca2+ concentration), temperature had the most pronounced effect on subunit exchange (30). The exchange rate of αA-crystallin subunits as monitored by fluorescence resonance energy transfer was facilitated by a temperature shift from 37 to 42°C. Several other reports indicate that high temperatures induce structural transitions in α-Hsp complexes (57, 250, 253, 282, 335, 338). A temperature increase triggers the exposure of hydrophobic residues, a structural reorganization that is thought to promote both subunit exchange and binding of unfolded proteins. Hetero-oligomers are probably more susceptible to temperature-driven conformational changes than are homo-oligomers since it was shown that complexes between Hsp27 and αB-crystallin were disrupted at 44°C (367). Complete reconstitution of mixed complexes occurred during recovery at 37°C.
Various posttranslational modifications, including phosphorylation, deamidation, acetylation, and glycosylation, have been detected for mammalian α-Hsps (11, 62, 71, 101, 193). Phosphorylation on one or more serine residues occurs in different tissues and in response to a wide array of environmental stimuli such as heat, arsenite, and growth factors. In the context of oligomerization, it is notable that phosphorylation often is associated with changes in the oligomeric structure of α-Hsp complexes. The correlation between phosphorylation, oligomer formation, and chaperone activity differs between individual α-Hsps (71, 193). However, in most cases, phosphorylation is associated with a reduction of the multimeric size. Hsp27, Hsp20, and αB-crystallin complexes are downsized by phosphorylation (17, 136, 145, 168, 259). Phosphorylation-induced dissociation of Hsp27 and αB-crystallin concomitantly reduce chaperone activity (136, 259). Before phosphorylation of maize mitochondrial Hsp22 was detected recently (191a), phosphorylation of α-Hsps was thought be an animal-specific process (314, 349).
Although lenticular α-crystallins have been the subject of intense investigation for many years, high-resolution structures are still unavailable. The dynamic quatenary structure of these proteins and numerous posttranslational modifications are thought to be the reason for their intrinsic resistance to crystallization trials (101). Numerous and in part controversial structural models have been proposed on the basis of known physicochemical properties of α-crystallins. Several competing three-layer models with variable numbers of subunits, a micelle-like structure, a “pitted-flexiball,” a “bean with tentacles,” and a GroEL-type complex are among the hypothetical models (42, 78, 101, 295, 336).
Microscopic examination of negatively stained samples revealed roughly spherical complexes for many members of the α-crystallin family, e.g., for mouse Hsp25, yeast Hsp26, human Hsp27, pea Hsp18.1 and Hsp17.7, Bradyrhizobium japonicum HspB and HspC, and Methanococcus jannaschii Hsp16.5 72, 74, 112, 156, 174, 175, 259; Studer et al., submitted). As mentioned above, cryo-EM images showed nonameric triangles of Mycobacterium tuberculosis Hsp16.3, a structural organization presently unique among α-Hsps (44). Three-dimensional reconstruction of cryo-EM images of human αB-crystallin, native bovine α-crystallin, human Hsp 27, and M. jannaschii Hsp16.5 visualized spherical complexes with an inner cavity (107, 108). The overall picture of the latter protein thus obtained closely matches its known crystal structure (155).
Whereas the first 32 residues of M. jannaschii Hsp16.5 are highly disordered in the crystal, the structure from residue 33 onwards, including the entire α-crystallin domain (residues 46 to 135) and the C-terminal extension (136 to 147), could be determined at 2.9 Å resolution (155). Twenty-four subunits are arranged with octahedral symmetry in a spherical complex containing eight triangular and six square openings (Fig. (Fig.5A).5A). The outer and inner diameters of the hollow sphere are around 120 and 65 Å, respectively. Each monomer consists of 10 β-strands and 2 short helices (Fig. (Fig.2).2). The core of Hsp16.5 adopts an immunglobulin-like fold consisting of two β-sheets that are packed as parallel layers. β1, β7, β5, and β4 form one β-sheet, and β2, β3, β9, and β8, together with β6 of a neighboring subunit, form the other β-sheet (Fig. (Fig.5B).5B). The donated strand is located in the center of the α-crystallin domain (Fig. (Fig.2).2). Each subunit in the complex makes extensive contacts with other subunits via hydrogen bonds as well as hydrophobic and ionic interactions. The short C-terminal extension is oriented toward the outside of the shell and interacts with β4 and β8 of a neighboring subunit. Although the size of the windows on the surface of the sphere would allow the passage principally of small molecules and unfolded polypeptide chains, it is unlikely that client proteins of Hsp16.5 are housed in the central cavity. Several lines of evidence, including them the presence of internal density in the Hsp16.5 shell in cryo-EM images, strongly indicate that the interior of Hsp16.5 and other α-Hsp complexes is filled with the disordered N-terminal region (107, 155, 182).
What does the Hsp16.5 structure tell us about the possible structure of other members of the α-crystallin family? The high-resolution structure of complexes that consist of 9, 12, 16, 32, or another number of subunits will certainly deviate from the 24-mer of Hsp16.5. Nevertheless, principal features of the Hsp16.5 structure might pertain to other α-Hsps, even if they do not form spherical assemblies. This assumption is nicely supported by the recently solved crystal structure of wheat Hsp16.9 (338a). The structures of monomeric and dimeric subparticles in the Hsp16.5 and Hsp16.9 complexes are very similar. Nevertheless, the overall quaternary structures are different. Wheat Hsp16.9 assembles not into spherical complexes but into a dodecameric double disk. Circular dichroism studies and secondary-structure predictions indicate that other α-Hsps also consist predominantly of β-sheets (32, 181, 202, 215, 282). It is important to note, however, that many residues involved in subunit contacts of M. jannaschii Hsp16.5 are not conserved in other family members (155). Most strikingly, the region around β6, which is intimately involved in monomer-monomer interactions, is extremely variable among α-Hsps or even absent, depending on the gap positioning in a given sequence alignment (compare Fig. Fig.22 and the alignment in reference 155). Despite the low sequence identity, a β-sandwich-like organization similar to that in the M. jannaschii protein was also demonstrated in the α-crystallin domains of αA-crystallin, Hsp27, and M. tuberculosis Hsp16.3 by site-directed spin labeling (22, 162). The β-strands of M. jannaschii Hsp16.5 and of αA-crystallin are illustrated at the top and bottom of Fig. Fig.2,2, respectively. Such comparative analyses show that the immunoglobulin-like fold of α-Hsp monomers is highly conserved. The divergence in the primary amino acid sequence, in particular in the flanking N- and C-terminal regions, most probably is responsible for the amazing differences in size, symmetry, and dynamics of the actual oligomeric structures.
Regions Responsible for Oligomerization
α-Crystallin domain.
The structural data outlined above leave little doubt that the α-crystallin domain is engaged in extensive subunit-subunit contacts. Congruent is the finding that a genetically engineered human αB-crystallin comprising only the α-crystallin domain forms a dimer (81). Yeast two-hybrid system analyses provide genetic evidence for interactions in the α-crystallin domain (27, 157, 168, 190, 359). The conserved motif A-x-x-x-n-G-v-L (Fig. (Fig.2)2) toward the C-terminal end of the α-crystallin domain was identified as an important determinant for the interaction of yeast Hsp42p (359). Efforts to identify individual amino acid residues involved in subunit interaction and/or chaperone activity by point mutagenesis had limited success owing to the astounding robustness of α-crystallins to limited perturbations (63, 128, 162, 218, 295). Although some point mutations resulted in significantly enlarged assemblies, chaperone efficiency was barely affected (128, 295).
Interestingly, two disease-related point mutations of a highly conserved arginine at an equivalent position in αA-crystallin (R116C) and αB-crystallin (R120G) introduce functionally relevant structural alterations (32, 50, 166, 244, 288). The αA-crystallin mutation occurs in patients suffering from hereditary cataracts. The αB-crystallin mutation causes desmin-related myopathy, a neuromuscular disease characterized by the accumulation of cytoplasmic inclusion bodies containing the defective αB-crystallin with the filament protein desmin. The mutated arginine of αA-and αB-crystallin is located in β-strand C3 (Fig. (Fig.2).2). It corresponds to an arginine in β7 of Methanococcus jannaschii Hsp16.5 and is moderately conserved throughout other α-Hsps. The arginine exchange derivatives have an oligomeric size twice to four times as large as the authentic proteins. Cryo-EM images of R120G-αB-crystallin revealed an irregular shape that lacks a well-defined central cavity (32). The conformational changes in R116C-αA-crystallin and R120G-αB-crystallin coincide with significantly reduced chaperone activity (32, 50, 166, 244, 288). The equivalent mutation (R100C) in Mycobacterium tuberculosis Hsp16.3 resulted in a protein that had only 40% of the wild-type chaperone activity (22). In contrast to the human α-crystallin proteins, the arginine exchange in Hsp16.3 resulted in a reduced complex size. Cysteine substitutions of S91, E92, F93, and Y95 also led to dissociation of the nonameric complex into smaller oligomers. This indicates that the region including and preceding the R100 residue serves as interface for the assembly of the trimeric building blocks of Hsp16.3. All other single-cysteine mutants between position 91 and 105 had no impact on oligomerization and chaperone activity.
N-terminal region.
A second important conclusion can be drawn from the dimeric state of the isolated α-crystallin domain mentioned above (81). Obviously, the central domain alone is not sufficient for the formation of higher-order structures. To assess the role of the N-terminal region and the C-terminal extension in α-Hsp assembly, the four Hsp12 proteins of Caenorhabditis elegans have been investigated. They are the smallest naturally occurring representatives of the α-crystallin family and are reduced to the α-crystallin domain preceded by an exceptionally short N-terminal region of 25 or 26 residues (160, 181). Although Hsp12.6 eluted as a dimer during size exclusion chromatography, sedimentation velocity experiments revealed a monomeric protein (181). Evidently, this result does not support any contribution of the α-crystallin domain to dimerization and subsequent oligomer assembly. In contrast, Hsp12.2 and Hsp12.3, two other miniature α-crystallin-type proteins of C. elegans, readily formed complexes up to tetramers (160). Neither of the Hsp12 proteins had detectable chaperone activity in vitro (160, 181). Their expression is developmentally regulated and unaltered by stress conditions. Since it is assumed that these proteins have specialized functions independent of oligomerization and chaperone activity, they may not be the best choice for drawing general conclusions on requirements for complex formation. Hsp16-2, yet another α-crystallin member of C. elegans, served as alternative model protein for studies on multimerization (182). The α-crystallin domain of this heat-inducible protein is flanked by a typical N-terminal region (41 residues) and a C-terminal extension (22 residues). Furthermore, purified Hsp16-2 is a classical chaperone that prevents thermally and chemically induced protein aggregation. The recombinant protein occurred in two subpopulations consisting of approximately 14 and 24 subunits. N-terminally truncated versions lacking 15, 32, or 44 amino acids failed to form native-like complexes, but trimeric and tetrameric species were discernible after cross-linking (182). Neither of the truncated Hsp16-2 proteins had chaperone activity. These studies clearly established a critical role of the N-terminal region in the assembly of low-molecular-mass species into functional high-molecular-mass complexes.
Since there is considerable deviation in the N-terminus of α-Hsps (Fig. (Fig.2),2), it is difficult to define the exact upper and lower limits of sequence length and the amino acid composition required for proper assembly of multimeric complexes. Human αA-crystallin devoid of the first 20 amino acids retained its high-molecular-mass structure, whereas a truncation of 56 residues reduced the complex to trimers or tetramers (31). The examination of truncated versions of Bradyrhizobium japonicum HspH (class A) and HspF (class B) also demonstrated that clipping off a few residues from the N terminus was tolerated without obvious defects in oligomerization and chaperone function whereas the removal of more than 5 to 10 amino acids was deleterious to both activities (Studer et al., submitted).
Interestingly, the N termini of certain α-Hsps can be remarkably insensitive to sequence extensions. Adding a tail of 4 -kDa that contains a hexahistidine tag to the N terminus of C. elegans Hsp16-2 did not disturb its multimerization capacity (182). The observation that the tagged protein bound to nickel-chelate affinity resin only in the presence of urea suggested that the N terminus is not exposed but sequestered in the interior of the complex. When maltose-binding protein (42 kDa) was added to the N terminus of αB-crystallin, the fusion protein still associated into high-molecular-mass oligomers that displayed full chaperone activity (215). This intriguing feature demonstrates that there is sufficient space in the cavity of the mammalian complex to accommodate N termini of various lengths. In contrast, the N termini of plant α-Hsps seem more sensitive to sequence additions. Fusion of glutathione S-transferase (29 kDa) to tobacco Hsp18 blocked oligomer formation at the dimeric stage (297).
C-terminal extension.
Whereas the importance of a largely intact N-terminal domain is well documented, the exact contribution of the C-terminal extension to complex formation is debated. Much like the N-terminal region, the length and sequence of the individual C-terminal ends vary considerably (Fig. (Fig.2).2). Point mutations or amino acid insertions in the last 4 residues of bovine αA-crystallin had little effect on the molecular mass of the complex (294). With one exception, chaperone activity was not disturbed when a hydrophobic tryptophan residue was introduced. The complete removal of the C-terminal extension from C. elegans Hsp16-2 had little impact on oligomerization and chaperone ability (182). The complexes obtained were slightly larger than wild-type complexes and readily precipitated after freeze-thawing. This was taken as evidence that one function of the C-terminal tail is to solubilize the α-Hsp complex. Mouse Hsp25 without its C-terminal extension also showed a normal oligomeric mass and suppressed thermal aggregation of CS (186). Surprisingly, the protein was unable to prevent DTT-induced precipitation of α-lactalbumin, implying that its flexible C-terminal tail, although not involved in oligomerization, is required for chaperone activity with certain substrates.
The oligomeric status of several other α-Hsps is considerably more sensitive to alterations in their C-terminal extensions. In line with the contention that the carboxyl end acts as solubilizing agent of α-Hsp complexes is the intrinsic insolubility of human αA-crystallin with the last 17 amino acids deleted (8). Precipitation goes along with markedly reduced chaperone activity. Comparable results were reported for Xenopus Hsp30C. Deletion of 25 amino acids from the carboxyl end resulted in reduced solubility and impaired chaperone function (82).
Reports on plant and bacterial α-Hsps demonstrate that the correct assembly into high-molecular-mass complexes depends on their carboxy termini. C-terminally shortened pea Hsp17.7 variants lacking 3, 5, or 10 amino acids were defective in the formation of full-size oligomers. In contrast to wild-type-like 250-kDa complexes, they formed assemblies of approximately 130, 100, and 67 kDa, respectively (157). Only small complexes, probably dimers, were detected when C-terminally truncated B. japonicum α-Hsps lacked the conserved I-X-I motif (sequences are given in Fig. Fig.2).2). Even the single replacement of either isoleucine by alanine completely impaired multimerization and consequently chaperone activity (Studer et al., submitted). This finding assigns an important structural role to this motif that is present in many, but not all, bacterial α-Hsps. The comparatively short extension of M. jannaschii Hsp16.5 carries both isoleucines followed by just one other residue (glutamic acid; Fig. Fig.2).2). The crystal structure shows that the tail reaches out of the sphere and that both isoleucines are involved in hydrophobic interactions with neighboring subunits (155). The C-terminal tail of wheat Hsp16.9 plays a similar critical role in stabilization of the oligomer (338a). Mutational studies of Hsp16.5 or Hsp16.9 have not been carried out. However, it is reasonable to assume that point mutations in the carboxyl end would destabilize and dissociate the complexes.
How can the discrepancies between reports concerning the role of the C-terminal extension be reconciled? Obviously, oligomerization is a very complicated process in which the actual requirements for individual α-Hsps might well be different. At least some bacterial α-Hsps are known to form highly ordered structures, in contrast to their polydisperse mammalian counterparts (44, 74, 107, 155). The C-terminal ends of M. jannaschii Hsp16.5 and of wheat Hsp16.9 are rigid and amenable to crystal structure determination (155, 338), whereas the tail of mammalian α-crystallin-type proteins reportedly is highly flexible (42). It is therefore likely that bacterial (and plant?) α-Hsps are more susceptible to mutational alterations. The exact positioning of all three functional regions might be more critical for the correct assembly of α-Hsps from these organisms. In this respect, it is interesting that more than 150 single-cysteine mutations in human αA-crystallin and 20 mutations in Hsp27 did not result in complex dissociation (22). On the other hand, 6 of 15 mutations in M. tuberculosis Hsp16.3 severely interfered with the assembly of native-like complexes. This comprehensive data set implies that only assemblies that are very dynamic can accommodate various point mutations or truncations without deleterious effects. It might therefore be worthwhile to carry out systematic site-directed mutagenesis studies on bacterial and plant α-Hsps.
Substrate-Binding Sites
The previous sections repeatedly emphasized the stringent coupling of complex formation and chaperone activity. Only certain oligomeric states, which vary among α-Hsp species, seem to orient interactive surfaces properly to promote substrate binding. Since the exposure of hydrophobic regions is characteristic of (un)folding intermediates, it has been surmised that hydrophobicity is an important parameter for chaperone-substrate interaction. In keeping with this conjecture is the finding that the chaperone efficiency of α-crystallins correlates with their degree of hydrophobicity. Far-UV circular dichroism and labeling with the fluorescent dye 1-anilino-8-naphthalene sulfonate (ANS) revealed that αB-crystallin has a greater content of α-helices and is more hydrophobic than αA-crystallin (57, 311). These structural features coincide with higher chaperone activity, indicating that hydrophobic interactions play an important role in substrate interaction. Furthermore, it has been reported that the temperature-driven exposure of hydrophobic surfaces in α-crystallin is accompanied by enhanced chaperone activity (250, 253). A temperature increase within the physiological range between 22 and 45°C triggered the exposure of buried hydrophobic regions in pea Hsp18.1, as was shown by the progressive increase of 1,1′-bi(4-anilino)naphthalene-5,5′-disulfonic acid (bis-ANS) incorporation (175). In the same temperature frame, E. coli IbpB undergoes similar conformational changes that alter surface hydrophobicity (282).
A number of studies made use of ANS, bis-ANS, or related small aromatic molecules to photolabel and subsequently localize potential substrate-binding sites in α-crystallin-type proteins. It is presumed that the regions interacting with these substances and with substrate proteins are identical for several reasons. First, preincubation of denatured alcohol dehydrogenase (ADH) with bovine α-crystallin or malate dehydrogenase (MDH) with pea Hsp18.1 blocked photoincorporation of the label (175, 280). Conversely, the binding of bis-ANS reduced the chaperone activity of α-crystallins (279, 293). Finally, regions identified by bis-ANS labeling overlapped with sites that cross-linked to substrate proteins (278, 281). Taken together, these data indicate that fluorescent probes and substrate proteins have common binding sites implicated in the chaperone activity of α-Hsps.
The outcome of photolabeling experiments with different α-Hsps varies. Incorporation of bis-ANS into rat αB-crystallin was restricted to the N-terminal domain (293). The labeled chaperone had considerably lower activity in the insulin assay than did untreated αB-crystallin, suggesting that a substrate-binding domain had been targeted by the label. Incorporation of fluorescent dyes into the amino-terminal region was also observed in bovine αA-crystallin and in pea Hsp18.1 (175, 280). The initial residues at the N terminus of Hsp18.1 and a short patch proximal to residue 50 of bovine αA-crystallin (QSLFR; highlighted in yellow in the human sequence in Fig. Fig.2)2) were photolabeled. The exchange of two conserved phenylalanines (F24 and F27) near the N terminus of αB-crystallin led to chaperone deficiency, although the oligomeric properties were not grossly changed (247). This result can be taken as further evidence that the N-terminal region of α-crystallin contributes to substrate binding. It should be noted, however, that this result is disputed and that other studies showed no discernible chaperone defect of the phenylalanine exchange derivatives (63, 128).
In contrast to the work on rat αB-crystallin, additional bis-ANS labeling was demonstrated in the α-crystallin domain of bovine αA- and αB-crystallins and of pea Hsp18.1 (175, 280). The corresponding peptides in the human α-crystallin proteins and the sequence in Methanococcus jannaschii Hsp16.5 equivalent to the region identified in Hsp18.1 are shown in yellow or green in Fig. Fig.2.2. Interestingly, the deduced substrate-binding site of Hsp16.5 maps in a loop that links β3 and β4. The crystal structure indicates that this loop is surface exposed and therefore well suited for protein-protein interactions (155). Several residues in this loop are involved in intersubunit contacts (79, 155). Likewise, in wheat Hsp16.9, several oligomerization interfaces coincide with putative substrate-binding sites, which led to the proposal that heat-induced chaperone activity is triggered by dissociation of the α-Hsp complex (338a). An intriguing feature of the presumed substrate-binding regions is the presence of several charged residues (Fig. (Fig.2).2). It has been proposed that such residues serve to generate optimal spacing of nonpolar residues and aid in hydration of the region (175). It is also conceivable that the chaperone and substrate interact via charged residues. Ionic pairing in addition to hydrophobic interactions might be useful for strengthening the stability of the chaperone-substrate complex, in particular when long-term storage of unfolded polypeptides is desired, as it is in the eye lens. Aside from their potential role in substrate binding, negative charges in the α-crystallin domain seem to be important to establish electrostatic interactions that stabilize the chaperone complex (27).
Cross-linking studies with denatured ADH or mellitin, a 2.8-kDa hydrophobic polypeptide, to bovine αA- and αB-crystallins disclosed similar sites to those defined by bis-ANS labeling (278, 281) (Fig. (Fig.2).2). Notably, the regions of αB-crystallin that generated a cross-link to ADH or mellitin were in close proximity but not identical. Two ADH-binding sites were located between residues 57 and 69 and residues 93 and 107, whereas the single mellitin-binding site encompasses amino acids 75 to 82. Whether different client proteins are indeed sequestered to different chaperone sites in α-Hsps remains to be established. The fact that pre-incubation of αB-crystallin with insulin outcompeted chaperone activity against α-lactalbumin suggests that the binding sites are at least partially overlapping (305). Residues highlighted in green in Fig. Fig.22 were identified by both the bis-ANS and cross-linking techniques (278, 280, 281). They cluster in an area corresponding to β3 to β5 in M. jannaschii Hsp16.5. Most strikingly, a synthetic 19-amino-acid peptide (KFVIFLDVKHFSPEDLTVK; residues 70 to 88 in αA-crystallin) prevented thermal aggregation of ADH, although with eightfold lower efficiency than did full-length αA-crystallin (281). This peptide also bound bis-ANS, strengthening the claim that bis-ANS-labeling sites and substrate-binding regions can be identical. The fact that Phe71, the second residue of that peptide, is essential for chaperone activity of rat αA-crystallin, lends additional support to the relevance of this region (266a). Although the participation of other regions cannot be excluded, it clearly emerges from these studies that the N terminus of the α-crystallin domain constitutes an important functional element for chaperone activity.
Numerous light-scattering studies demonstrate that α-Hsps act as molecular chaperones in the sense that they interact with target proteins and prevent their precipitation (44, 72, 74, 112, 127, 138, 156, 174, 175, 182, 202, 215, 262, 282, 310). α-Hsps are able to capture thermally or chemically denatured model substrates. Binding to the chaperone does not protect a substrate from its inactivation. The inactivation kinetics of several test enzymes was similar regardless of whether α-Hsps were present (44, 72, 174, 262). Moreover, MDH complexed with Hsp18.1 is hypersensitive to proteinase K treatment whereas MDH alone is resistant (175). Both findings indicate that α-Hsps recognize and sequester unfolded structures rather than native proteins. Bound substrates are thought to be in a flexible, molten-globule-like state in which unfolding is incomplete and secondary structure is preserved (55, 56, 187, 249). The fluorescence characteristics of tryptophan residues in α-crystallin-bound substrates were closer to those of native proteins than to those of fully unfolded ones (56). This is consistent with the idea that α-Hsps specifically recognize labile unfolding intermediates that occur early in the denaturation pathway.
In contrast to the GroEL complex that accommodates one or two substrate molecules per 14 subunits (111), α-Hsp assemblies have a much higher binding capacity. Many studies document that a molar (monomeric) chaperone to substrate ratio of 1:1 suffices to almost completely abolish light scattering (44, 72, 112, 127, 138, 310). Substrate-binding efficiency can vary depending on the temperature and model protein investigated. A 40:1 molar ratio of Methanococcus jannaschii Hsp16.5 to CS was necessary to prevent light scattering at 40°C (156). However, at 80°C, a temperature close to the growth optimum of 85°C for this organism, it protected single-chain monellin at a 1:1 molar ratio. Size exclusion chromatography demonstrated that pea Hsp18.1 could be saturated with 12 MDH molecules per dodecamer whereas it bound only an average of 0.25 CS subunit per monomer (175). The relative binding capacity of α-crystallin for DTT-sensitive proteins ranged from 2:1 (α-crystallin to insulin or α-crystallin to α-lactalbumin), over 8:1 (α-crystallin to bovine serum albumin) to 10:1 (α-crystallin to ovotransferrin) (188). The molecular masses of these four model substrates are 5.7, 14, 66, and 78 kDa, respectively. The clear correlation between low molecular mass of a substrate and high binding capacity of the chaperone implies that steric factors dictate the number of molecules that can be positioned on the surface of the α-Hsp complex. The finding that the rate of subunit exchange of αA-crystallin was markedly reduced on interaction with large target proteins indicates also that extended polypeptides interact simultaneously with multiple subunits of the chaperone (30).
Once formed, the chaperone-substrate complex is very stable. For instance, E. coli IbpA and IbpB bound tightly to inclusion bodies formed during heterologous protein production, a feature that led to their designation as “inclusion body-associated proteins” (6). Both proteins could also be recovered from endogenous E. coli proteins that had aggregated during heat treatment (170). In vitro, CS remained stably associated with Hsp25 for several hours (72). Likewise, complexes formed between Hsp18.1 and diverse substrates were stable for weeks at room temperature and were not disrupted by addition of ATP or salt or by storage at 4°C (175). Irreversible binding of unfolded proteins might be the only activity of lenticular α-crystallins, since there is no protein turnover in the eye lens. However, it is important to emphasize that polypeptides recruited by α-Hsps are not necessarily stuck in a dead-end conformation. CS could be released from Hsp25 and reactivated by the addition of oxaloacetate, a substrate and stabilizing ligand of the enzyme (72). Thus, the substrate is bound in a refoldable state. The overall picture that emerges is that α-Hsps act as very efficient molecular sponges that collect and immobilize denatured proteins on their way to irreversible aggregation. The storage of up to equimolar amounts of partially folded polypeptides provides a large reservoir of protein material that can be recycled under permissive conditions.
The chaperone action of α-Hsps described above is generally believed to be ATP independent (18, 137, 349). The addition of ATP did not enhance the chaperone activity of E. coli IbpB, Mycobacterium tuberculosis Hsp16.3, murine Hsp25, or pea Hsp18.1 and Hsp17.7 (44, 72, 174, 341). On the other hand, it has been proposed that the cellular ATP concentration modulates the chaperoning efficiency of certain α-Hsps. Light scattering of CS was suppressed by human αB-crystallin twice as efficiently in the presence of 3.5 mM ATP (216). Nonhydrolyzable ATP analogs had no stimulatory effect. Tryptophan fluorescence studies and mass spectrometry of tryptic digests of the chaperone demonstrated ATP-dependent structural modifications in the α-crystallin domain, which might influence its functionality (216, 217). ATP-enhanced chaperone activity of αB-crystallin was independently confirmed in experiments with the bovine protein (297). Parallel measurements performed with tobacco Hsp18 showed that ATP had an adverse effect; it reduced chaperone activity in the CS protection assay in a concentration-dependent manner. Again, conformational changes seem to be responsible for the ATP effect. In the presence of ATP, bis-ANS labeling of Hsp18 was reduced. Moreover, quenching of intrinsic tryptophan fluorescence suggested that Hsp18 has a more compact conformation in the presence of ATP. Whether these observations are of physiological relevance is a matter of speculation. Incidentally, the ATP concentration in the eye lens is higher than in most other tissues. Thus, stimulation of α-crystallin by ATP might be important for optimal chaperone activity in the lens (216). Abundant ATP in the plant cytosol is indicative of the absence of stress, which would make the action of α-Hsps obsolete. Under severe stress conditions when the ATP concentration drops, chaperones of the Hsp70 and Hsp60 families will not function efficiently. Simultaneous activation of α-Hsps would provide an elegant mechanism to coordinate the activity of ATP-dependent and ATP-independent chaperones by the availability of the nucleotide (297).
What is a cell going to do with the reservoir of folding-competent polypeptides that are deposited on the surface of α-Hsps? Although release and reactivation of bound substrates has been described, it is not a very productive process (72, 138, 216, 297, 341). When rabbit reticulocyte lysate, a rich source of chaperones, was added to luciferase complexed with either pea Hsp18.1 or bovine α-crystallin, enzyme activity was restored much more efficiently (175, 346). The stimulatory effect was strictly dependent on ATP. Since wheat germ extract had a similar, albeit weaker, effect on reactivation of Hsp18.1-bound luciferase with respect to that of rabbit reticulocyte lysate, it was proposed that a widely conserved ATP-dependent chaperone would assist in refolding (175). The first hint that this component might be Hsp70 (DnaK) came from the finding that addition of this chaperone together with ATP enhanced reactivation of Hsp25-bound CS (72). The observation that an E. coli ibpAB mutation exerted a deleterious growth defect at 42°C only in combination with a mutation in dnaK (dnaK756) but not with a mutation in groESL (groES30) implied a close cooperation with the DnaK machinery but not with GroESL in vivo (319). The structure of HSGs with α-Hsps in their inner core and Hsp70 on the surface is a further indication that the two chaperones work hand in hand (296).
Detailed biochemical studies confirmed that DnaK is the specific release factor for α-Hsp-bound substrates (176, 325, 341, 346). Refolding of heat-denatured MDH stabilized by IbpB was slow in the absence of other chaperones or in the presence of GroESL (341). Supplementation of MDH-IbpB with the DnaK system enhanced refolding significantly. Further recovery could be achieved by combining the DnaK and GroEL machineries. Gel filtration analyses demonstrated a sequential transfer of MDH from IbpB to DnaK and then to GroEL (341). Fig. Fig.6A6A outlines the fate of substrate proteins bound to α-Hsps. It is assumed that only a small portion, if any, will refold spontaneously. The majority are being transferred to the DnaK machinery. One fraction will be refolded by DnaK, whereas another fraction must be passed on to GroEL before it can be refolded. In vitro, between 40 and 80% of MDH or lactate dehydrogenase was refolded by the combined action of IbpB, DnaK, and GroEL (341). The incomplete recovery may indicate that some enzyme escapes from chaperone-mediated protection by irreversible aggregate formation.
FIG. 6.
FIG. 6.
Function of α-Hsps in a multichaperone network. (A) Sequential transfer of α-Hsp-bound substrates for further processing. (B) Schematic representation of the cellular multichaperone network. For details, see the text.
The position of α-Hsps in the context of a dynamic and synergistic multichaperone network in a stressed cell is depicted in Fig. Fig.6B.6B. Without α-Hsps, denatured proteins either can be refolded by the major chaperone machineries or will form insoluble aggregates destined for degradation. The presence of α-Hsps offers an alternative pathway that captures unfolding intermediates before they aggregate. The cell can make use of this large reservoir of folding-competent proteins whenever more suitable refolding conditions have been reestablished. It is interesting that IbpB displayed lower affinity to denatured MDH than did DnaK and GroEL (341). Hence, immediate refolding of denatured proteins by DnaK or GroEL seems to be the preferred option. The initial choice of chaperone probably depends on the availability. In this sense, α-Hsps serve as emergency chaperones under circumstances when DnaK and GroEL are occupied and/or when ATP becomes limiting. α-Hsps then reduce the flow of nonnative proteins toward aggregation and redirect them to the folding pathway.
The fact that DnaK rather than GroEL is required for immediate steps in further processing implies that the latter has no access to α-Hsp-bound proteins. It is unclear whether this is because GroEL encloses substrates in its central cavity and DnaK binds them at the surface or whether the unfolded proteins are in a conformation that cannot be handled by GroEL for other reasons. For example, two typical features of DnaK substrates are large size and local aggregation (67, 196, 211). Another unsolved puzzle is that some hyperthermophilic archaea lack an apparent dnaK homologue but nevertheless have a α-Hsp gene (192). Thus, substrate delivery pathways other than the one outlined above may occur in nature.
Bearing in mind the central position of α-Hsps in protein quality control (Fig. (Fig.6),6), it is perplexing that E. coli ibpAB mutants do not accumulate more aggregates after heat shock than the wild type does (319) or that the addition of IbpB to E. coli extracts does not prevent heat-induced protein aggregation (211). The deletion of ibpA and ibpB in E. coli did not produce a stress-sensitive mutant strain. However, overexpression of both genes increased the resistance to heat and superoxide stress (158). Moreover, thermotolerance of E. coli could be enhanced by the expression of various heterologous α-Hsps (216, 247, 301, 362). In contrast to E. coli, the deletion of hsp16.6 in Synechocystis sp. strain PCC 6803 resulted in a clear growth defect after heat shock treatment (177, 178) and disruption of hsp18 in Streptomyces albus showed that the gene is required for thermotolerance at extreme temperatures (275). Thus, there is cumulative in vivo evidence that α-Hsps do play a physiological role in the protection against adverse conditions. In general, it is difficult to ascertain the relative contribution of individual chaperones to protein folding. The simultaneous action of multiple chaperones hampers the design and interpretation of experiments in a cellular context. This is why in vitro studies of chaperone research often have been much more rewarding than in vivo experiments.
Members of the α-Hsp family have been implicated in an ever-growing number of cellular activities. The by no means complete list includes eye lens transparency (33); thermotolerance (169, 171, 177, 198, 248, 261, 270, 332, 362); resistance to apoptosis (10, 35, 45, 199-201); cytoskeleton modulation (20, 104, 172, 184, 207, 232); prevention of amyloid formation (165, 307); human diseases (48); various developmental processes in animals (11, 118, 181, 185, 203), plants (349), and bacteria (115); protection against oxidative stress (109, 259); desiccation tolerance (354); protection of the photosynthetic apparatus (113, 221) or of mitochondrial NADH:ubiquinone oxidoreductase (complex I) (68, 69); microbial pathogenicity (2, 54, 228, 283, 342, 363, 365); symbiotic and pathogenic plant-microbe interactions (16, 226); metabolic shift from acid to solvent production (245, 267); protection against acid shock (2, 95, 106); and sporulation (120). It is tempting to assume that the functional importance of α-Hsps in all these processes lies exclusively in the general protection of other proteins. Although this interpretation may be valid for most of the examples given above, there is increasing evidence that α-Hsps are concerned with functions other than chaperoning. The interaction between αB-crystallin and a proteosomal subunit might suggest that α-Hsps facilitate not only refolding but also selective degradation of target proteins (26) (Fig. (Fig.66).
Several studies demonstrate an interaction between α-Hsps and nucleic acids. HSGs in plants and mammals harbor untranslated mRNAs (149, 237). It is not clear whether α-Hsps directly bind RNA or whether the coassembly occurs via other proteins recruited into the HSG. A potential indirect role of α-Hsps in the transient storage and protection of mRNA during stress-induced translation arrest is supported by two lines of evidence. First, there is a specific association of several ribonuclear proteins and the heat shock transcription factor HsfA2 with HSGs (149, 268). Second, Hsp27 specifically interacts with the translation factor eIF4G and thereby inhibits protein synthesis under heat shock conditions, which are unfavorable for translation of most cellular mRNAs (53). Other reports show that α-crystallin directly binds single-stranded and double-stranded DNA (246, 290). Helices in α-crystallin have been suggested to play a role in DNA binding (25). Taken together, these observations suggest that α-Hsps may have largely unexplored functions in nucleic acid metabolism.
Recently, a potential link between α-Hsps and membrane functions has received growing attention. The occurrence of α-Hsps in the cell periphery has been reported repeatedly, for instance in Stigmatella aurantiaca, Oenococcus oeni, M. tuberculosis, and E. coli (61, 116, 142, 170, 173, 191). However, since α-Hsps are routinely detectable by standard two-dimensional gel electrophoresis (3, 95, 106, 205, 219, 226, 365), it appears that at least a major fraction is soluble and, if at all, only loosely attached to membranes. Studies with lens plasma membranes suggest that a subfraction of α-crystallin, once attached to the membrane, becomes irreversibly buried in the membrane bilayer (49). A critical role of α-Hsps in controlling the physical state of membranes has been established with Hsp17 (Hsp16.6) from Synechocystis strain sp. PCC 6803. This photosynthetic cyanobacterium forms irregular thylakoid membranes and evolves less oxygen when hsp17 is inactivated (177, 178). The interpretation that Hsp17 is an important stabilizer of photosynthetic membranes is supported by the fact that the majority of heat-induced Hsp17 associates with thylakoid membranes (125). Altering the membrane physical state by administration of the fluidizer benzyl alcohol enhanced the thermosensitivity of Synechocystis cells. In parallel, the threshold temperature required for induction of heat shock genes, including dnaK, groESL, and hsp17, was reduced. The close correlation between membrane order and heat shock response led to the hypothesis that membranes act as cellular thermometer from which stress is sensed and transduced into signaling pathways that activate heat shock gene expression (125, 344). Two features make membranes the prime candidate for monitoring thermal changes. First, they are among the first cellular structures that encounter external stress. Second, membrane fluidity is very sensitive to temperature variations, at both high and low temperatures (343, 344). Maintaining membrane integrity under stress conditions is an important job of Hsp17, as was shown by a combination of genetic and in vitro approaches. Fluorescence anisotropy measurements with isolated thylakoid membranes revealed that membrane fluidity was higher in preparations from an hsp17 mutant than in wild-type membranes (325). The interaction between Hsp17 and large unilamellar vesicles made of synthetic or cyanobacterial lipids strongly increased the molecular order of the membranes. Penetration into the membrane hydrophobic core implies that Hsp17-membrane interactions are lipid mediated and are not due to membrane surface contacts. Lipid and substrate protein interaction seem to be mutually exclusive since the addition of lipids to an Hsp17-DnaK-GroEL refolding system strongly inhibited the reactivation of MDH (325). Under stress conditions, the cellular pool of α-Hsps is probably divided into a cytoplasmic subfraction responsible for regular chaperone activity and a membraneous subfraction involved in membrane stabilization. The most recent data demonstrate that specific lipid binding is not confined to cyanobacterial Hsp17 but also a feature of αB-crystallin (N. M. Tsvethova, I. Horvath, Z. Török, W. F. Wolkers, F. Tablin, E. Vierling, J. H. Gowa, and L. Vigh, submitted for publicatication). The precise nature of α-Hsp membrane interaction depends on the lipid composition and extent of fatty acid saturation. Most intriguingly, enhanced cell viability owing to the presence of α-Hsps has also been described during chilling (265, 266, 301). Membrane fluidity modulation by α-Hsps can fully explain a protective effect against both thermal extremes. While α-Hsps are able to rigidify membranes at high temperatures, they seem to fluidize saturated lipid species at low temperatures (Tsvethova et al., submitted).
In summary, α-Hsps seem to be very versatile protective agents. They play a dual role in protein and membrane protection and also might be involved in nucleic acid preservation. Chaperone research tends to overlook the fact that under stress conditions, the integrity of proteins is not the only thing at stake. Other macromolecules including nucleic acids and membranes will disintegrate at high temperatures if they are not protected immediately. In this context, it is interesting that GroEL has also been implicated in mRNA protection and membrane stabilization (59, 90, 326). Apparently, α-Hsps are not the only chaperones that help maintain the structural integrity of proteins, nucleic acids, and membranes.
α-Hsps constitute the most divergent Hsp family. Despite their limited monomeric size, they socialize with each other, with other chaperones, and with diverse substrates through a large number of interactions, by which they serve to protect cellular macromolecules. Although the chaperone activity of α-Hsps was discovered almost a decade ago, many fundamental questions concerning this function remain unanswered. A strict correlation between oligomerization and chaperone activity is widely accepted. However, the underlying mechanistic details of this relationship are poorly understood. Moreover, the α-Hsp regions that contact substrate proteins are far from being defined, as are the recognition sites in unfolded proteins. Even more remains to be learned about the recently uncovered functions of α-Hsps. It is virtually unknown whether oligomerization is a prerequisite for interactions with nucleic acids or lipids. The α-Hsp sites interacting with these molecules still need to be explored. They are most probably different from those that contact unfolded proteins.
Revealing unifying concepts for the structure and function of α-Hsps is complicated by the fact that individual family members deviate substantially in their amino acid sequence and quaternary structure. Any isolated finding concerning one α-Hsp cannot necessarily claim to be true for others. Importantly, representative examples from archaea, bacteria, plants, and animals are now being investigated in order to arrive at a comprehensive picture. Only the concerted efforts of genetic, biochemical, biophysical, and structural studies will help unravel the general features of α-Hsps and the peculiarities of individual family members.
Acknowledgments
I thank Hauke Hennecke for generous support and continuous interest in my research activities. Sonja Studer, Nicolas Lentze, Markus Obrist, and Hans-Martin Fischer are gratefully acknowledged for helpful comments on the manuscript and for their contributions to the ongoing α-Hsp project. The dedicated work from all past and present coworkers on this and related projects is highly appreciated. I am grateful to Laszlo Vigh and Christian Baron for communicating results prior to publication.
Work in my laboratory is financed by grants from the Swiss National Foundation for Scientific Research and the Swiss Federal Institute of Technology, Zürich, Switzerland.
1. Abgar, S., N. Yevlampieva, T. Aerts, J. Vanhoudt, and J. Clauwaert. 2000. Chaperone-like activity of bovine lens α-crystallin in the presence of dithiothreitol-destabilized proteins: characterization of the formed complexes. Biochem. Biophys. Res. Commun. 276:619-625. [PubMed]
2. Abu Kwaik, Y., and N. C. Engleberg. 1994. Cloning and molecular characterization of a Legionella pneumophila gene induced by intracellular infection and by various in vitro stress conditions. Mol. Microbiol. 13:243-251. [PubMed]
3. Abu Kwaik, Y., L. Y. Gao, O. S. Harb, and B. J. Stone. 1997. Transcriptional regulation of the macrophage-induced gene (gspA) of Legionella pneumophila and phenotypic characterization of a null mutant. Mol. Microbiol. 24:629-642. [PubMed]
4. Akiyama, Y., M. Ehrmann, A. Kihara, and K. Ito. 1998. Polypeptide binding of Escherichia coli FtsH (HflB). Mol. Microbiol. 28:803-812. [PubMed]
5. Akiyama, Y., T. Ogura, and K. Ito. 1994. Involvement of FtsH in protein assembly into and through the membrane. I. Mutations that reduce retention of a cytoplasmic reporter. J. Biol. Chem. 269:5218-5224. [PubMed]
6. Allen, S. P., J. O. Polazzi, J. K. Gierse, and A. M. Easton. 1992. Two novel heat shock genes encoding proteins produced in response to heterologous protein expression in Escherichia coli. J. Bacteriol. 174:6938-6947. [PMC free article] [PubMed]
7. Andersson, S. G. E., A. Zomorodipour, J. O. Andersson, T. Sicheritz-Ponten et al. 1998. The genome sequence of Rickettsia prowazekii and the origin of mitochondria. Nature 396:133-140. [PubMed]
8. Andley, U. P., S. Mathur, T. A. Griest, and J. M. Petrash. 1996. Cloning, expression, and chaperone-like activity of human αA-crystallin. J. Biol. Chem. 271:31973-31980. [PubMed]
9. Anfinsen, C. B. 1973. Principles that govern the folding of protein chains. Science 181:223-230. [PubMed]
10. Arrigo, A. P. 1998. Small stress proteins: chaperones that act as regulators of intracellular redox state and programmed cell death. Biol. Chem. 379:19-26. [PubMed]
11. Arrigo, A. P., and J. Landry. 1994. Expression and function of the low-molecular-weight heat shock proteins, p. 335-373. In R. I. Morimoto, A. Tissières, and C. Georgopoulos (ed.). The biology of heat shock proteins and molecular chaperones. Cold Spring Harbor Laboratory Press, Cold Spring Harbor, N.Y.
12. Babst, M., H. Hennecke, and H. M. Fischer. 1996. Two different mechanisms are involved in the heat-shock regulation of chaperonin gene expression in Bradyrhizobium japonicum. Mol. Microbiol. 19:827-839. [PubMed]
13. Bahl, H., H. Müller, S. Behrens, H. Joseph, and F. Narberhaus. 1995. Expression of heat shock genes in Clostridium acetobutylicum. FEMS Microbiol. Rev. 17:341-348. [PubMed]
14. Barbirz, S., U. Jakob, and M. O. Glocker. 2000. Mass spectroscopy unravels disulfide bond formation as the mechanism that activates a molecular chaperone. J. Biol. Chem. 275:18759-18766. [PubMed]
15. Bardwell, J. C. A., and E. A. Craig. 1988. Ancient heat shock gene is dispensable. J. Bacteriol. 170:2977-2983. [PMC free article] [PubMed]
16. Baron, C., N. Domke, M. Beinhofer, and S. Hapfelmeier. 2001. Elevated temperature differentially affects virulence, VirB protein accumulation, and T-pilus formation in different Agrobacterium tumefaciens and Agrobacterium vitis strains. J. Bacteriol. 183:6852-6861. [PMC free article] [PubMed]
17. Beall, A., D. Bagwell, D. Woodrum, T. A. Stoming, K. Kato, A. Suzuki, H. Rasmussen, and C. M. Brophy. 1999. The small heat shock-related protein, HSP20, is phosphorylated on serine 16 during cyclic nucleotide-dependent relaxation. J. Biol. Chem. 274:11344-11351. [PubMed]
18. Beissinger, M., and J. Buchner. 1998. How chaperones fold proteins. Biol. Chem. 379:245-259. [PubMed]
19. Bell, S. D., and S. P. Jackson. 1998. Transcription and translation in Archaea: a mosaic of eukaryal and bacterial features. Trends Microbiol. 6:222-228. [PubMed]
20. Benndorf, R., K. Hayess, S. Ryazantsev, M. Wieske, J. Behlke, and G. Lutsch. 1994. Phosphorylation and supramolecular organization of murine small heat shock protein HSP25 abolish its actin polymerization-inhibiting activity. J. Biol. Chem. 269:20780-20784. [PubMed]
21. Benov, L., and I. Fridovich. 1995. Superoxide dismutase protects against heat shock in Escherichia coli. J. Bacteriol. 177:3344-3346. [PMC free article] [PubMed]
22. Berengian, A. R., M. Parfenova, and H. S. Mchaourab. 1999. Site-directed spin labeling study of subunit interactions in the α-crystallin domain of small heat-shock proteins: comparison of the oligomer symmetry in αA-crystallin, Hsp27 and Hsp16.3. J. Biol. Chem. 274:6305-6314. [PubMed]
23. Blaszczak, A., M. Zylicz, C. Georgopoulos, and K. Liberek. 1995. Both ambient temperature and the DnaK chaperone machine modulate the heat shock response in Escherichia coli by regulating the switch between σ70 and σ32 factors assembled with RNA polymerase. EMBO J. 14:5085-5093. [PubMed]
24. Blattner, F. R., G. Plunkett, C. A. Bloch, N. T. Perna, V. Burland et al. 1997. The complete genome sequence of Escherichia coli K-12. Science 277:1453-1474. [PubMed]
25. Bloemendal, M., A. Toumadje, and W. C. Johnson. 1999. Bovine lens crystallins do contain helical structures: a circular dichroism study. Biochim. Biophys. Acta 1432:234-238. [PubMed]
26. Boelens, W. C., Y. Croes, and W. W. de Jong. 2001. Interaction between αB-crystallin and the human 20S proteasomal subunit C8/alpha7. Biochim. Biophys. Acta 1544:311-319. [PubMed]
27. Boelens, W. C., Y. Croes, M. de Ruwe, L. de Reu, and W. W. de Jong. 1998. Negative charges in the C-terminal domain stabilize the αB-crystallin complex. J. Biol. Chem. 273:28085-28090. [PubMed]
28. Reference deleted.
29. Booth, R. J., D. L. Williams, K. D. Moudgil, L. C. Noonan, P. M. Grandison, J. J. McKee, R. L. Prestidge, and J. D. Watson 1993. Homologs of Mycobacterium leprae 18-kilodalton and Mycobacterium tuberculosis 19-kilodalton antigens in other mycobacteria. Infect. Immun. 61:1509-1515. [PMC free article] [PubMed]
30. Bova, M. P., L. L. Ding, J. Horwitz, and B. K. Fung. 1997. Subunit exchange of αA-crystallin. J. Biol. Chem. 272:29511-29517. [PubMed]
31. Bova, M. P., H. S. Mchaourab, Y. Han, and B. K. K. Fung. 2000. Subunit exchange of small heat shock proteins—analysis of oligomer formation of αA-crystallin and Hsp27 by fluorescence resonance energy transfer and site-directed truncations. J. Biol. Chem. 275:1035-1042. [PubMed]
32. Bova, M. P., O. Yaron, Q. L. Huang, L. L. Ding, D. A. Haley, P. L. Stewart, and J. Horwitz. 1999. Mutation R120G in αB-crystallin, which is linked to a desmin-related myopathy, results in an irregular structure and defective chaperone-like function. Proc. Natl. Acad. Sci. USA 96:6137-6142. [PubMed]
33. Brady, J. P., D. Garland, Y. Duglas-Tabor, W. G. J. Robison, A. Groome, and E. F. Wawrousek. 1997. Targeted disruption of the mouse αA-crystallin gene induces cataract and cytoplasmic inclusion bodies containing the small heat shock protein αB-crystallin. Proc. Natl. Acad. Sci. USA 94:884-889. [PubMed]
34. Brans, A., A. Loriaux, B. Joris, and J. Dusart. 1996. Cloning and sequencing of the dnaK locus in Streptomyces coelicolor A3(2). DNA Sequence 6:179-184. [PubMed]
35. Bruey, J. M., C. Ducasse, P. Bonniaud, L. Ravagnan, S. A. Susin, C. Diaz-Latoud, S. Gurbuxani, A. P. Arrigo, G. Kroemer, E. Solary, and C. Garrido. 2000. Hsp27 negatively regulates cell death by interacting with cytochrome c. Nat. Cell Biol. 2:645-652. [PubMed]
36. Buchner, J. 1999. Hsp90 & Co.—a holding for folding. Trends Biochem. Sci. 24:136-141. [PubMed]
37. Buchner, J. 1996. Supervising the fold: Functional principles of molecular chaperones. FASEB J. 10:10-19. [PubMed]
38. Bukau, B. 1993. Regulation of the Escherichia coli heat-shock response. Mol. Microbiol. 9:671-680. [PubMed]
39. Bukau, B., E. Deuerling, C. Pfund, and E. A. Craig. 2000. Getting newly synthesized proteins into shape. Cell 101:119-122. [PubMed]
40. Bukau, B., and A. L. Horwich. 1998. The Hsp70 and Hsp60 chaperone machines. Cell 92:351-366. [PubMed]
41. Bult, C. J., O. White, G. J. Olsen, L. X. Zhou, R. D. Fleischmann, et al. 1996. Complete genome sequence of the methanogenic archaeon, Methanococcus jannaschii. Science 273:1058-1073. [PubMed]
42. Carver, J. A., and R. A. Lindner. 1998. NMR spectroscopy of α-crystallin. Insights into the structure, interactions and chaperone action of small heat-shock proteins. Int. J. Biol. Macromol. 22:197-209. [PubMed]
43. Caspers, G. J., J. A. M. Leunissen, and W. W. de Jong. 1995. The expanding small heat-shock protein family, and structure predictions of the conserved ‘α-crystallin domain'. J. Mol. E vol. 40:238-248. [PubMed]
44. Chang, Z. Y., T. P. Primm, J. Jakana, I. H. Lee, I. Serysheva, W. Chiu, H. F. Gilbert, and F. A. Quiocho. 1996. Mycobacterium tuberculosis 16-kDa antigen (Hsp16.3) functions as an oligomeric structure in vitro to suppress thermal aggregation. J. Biol. Chem. 271:7218-7223. [PubMed]
45. Charette, S. J., J. N. Lavoie, H. Lambert, and J. Landry. 2000. Inhibition of Daxx-mediated apoptosis by heat shock protein 27. Mol. Cell. Biol. 20:7602-7612. [PMC free article] [PubMed]
46. Chuang, S. E., and F. R. Blattner. 1993. Characterization of twenty-six new heat shock genes of Escherichia coli. J. Bacteriol. 175:5242-5252. [PMC free article] [PubMed]
47. Ciechanover, A. 1998. The ubiquitin-proteasome pathway: on protein death and cell life. EMBO J. 17:7151-7160. [PubMed]
48. Clark, J. I., and P. J. Muchowski. 2000. Small heat-shock proteins and their potential role in human disease. Curr. Opin. Struct. Biol. 10:52-59. [PubMed]
49. Cobb, B. A., and J. M. Petrash. 2000. Characterization of α-crystallin-plasma membrane binding. J. Biol. Chem. 275:6664-6672. [PMC free article] [PubMed]
50. Cobb, B. A., and J. M. Petrash. 2000. Structural and functional changes in the αA-crystallin R116C mutant in hereditary cataracts. Biochemistry 39:15791-15798. [PMC free article] [PubMed]
51. Cole, S. T., R. Brosch, J. Parkhill, T. Garnier, C. Churcher, et al. 1998. Deciphering the biology of Mycobacterium tuberculosis from the complete genome sequence. Nature 393:537-544. [PubMed]
52. Cole, S. T., K. Eiglmeier, J. Parkhill, K. D. James, N. R. Thomson, et al. 2001. Massive gene decay in the leprosy bacillus. Nature 409:1007-1011. [PubMed]
53. Cuesta, R., G. Laroia, and R. J. Schneider. 2000. Chaperone hsp27 inhibits translation during heat shock by binding eIF4G and facilitating dissociation of cap-initiation complexes. Genes Dev. 14:1460-1470. [PubMed]
54. Cunningham, A. F., and C. L. Spreadbury. 1998. Mycobacterial stationary phase induced by low oxygen tension: cell wall thickening and localization of the 16-kilodaltonα-crystallin homolog. J. Bacteriol. 180:801-808. [PMC free article] [PubMed]
55. Das, K. P., L. P. Choo-Sith, J. M. Petrash, and W. K. Surewicz. 1999. Insights into the secondary structure of non-native proteins bound to a molecular chaperone α-crystallin: an isotope-edited infrared spectroscopic study. J. Biol. Chem. 274:33209-33212. [PubMed]
56. Das, K. P., J. M. Petrash, and W. K. Surewicz. 1996. Conformational properties of substrate proteins bound to a molecular chaperone α-crystallin. J. Biol. Chem. 271:10449-10452. [PubMed]
57. Datta, S. A., and C. M. Rao. 1999. Differential temperature-dependent chaperone-like activity of αA- and αB- crystallin homoaggregates. J. Biol. Chem. 274:34773-34778. [PubMed]
58. Davidson, J. F., B. Whyte, P. H. Bissinger, and R. H. Schiestl. 1996. Oxidative stress is involved in heat-induced cell death in Saccharomyces cerevisiae. Proc. Natl. Acad. Sci. USA 14:5116-5121. [PubMed]
59. De Bruyn, J., K. Soetaert, P. Buyssens, I. Calonne, J. L. De Coene, X. Gallet, R. Brasseur, R. Wattiez, P. Falmagne, H. Montrozier, M. A. Laneelle, and M. Daffé 2000. Evidence for specific and non-covalent binding of lipids to natural and recombinant Mycobacterium bovis BCG Hsp60 proteins, and to the Escherichia coli homologue GroEL. Microbiology 146:1513-1524. [PubMed]
60. Deckert, G., P. V. Warren, T. Gaasterland, W. G. Young, A. L. Lenox, et al. 1998. The complete genome of the hyperthermophilic bacterium Aquifex aeolicus. Nature 392:353-358. [PubMed]
61. De Jong, W. W., G. J. Caspers, and J. A. M. Leunissen. 1998. Genealogy of the α-crystallin-small heat-shock protein superfamily. Int. J. Biol. Macromol. 22:151-162. [PubMed]
61. Delmas, F., F. Pierre, F. Coucheney, C. Divies, and J. Guzzo. 2001. Biochemical and phyiological studies of the small heat shock protein Lo18 from the lactic acid bacterium Oenocucoccus oeni. J. Mol. Microbiol. Biotechnol. 3:601-610. [PubMed]
62. Derham, B. K., and J. J. Harding. 1999. α-Crystallin as a molecular chaperone. Prog. Retin. Eye Res. 18:463-509. [PubMed]
63. Derham, B. K., M. A. van Boekel, P. J. Muchowski, J. I. Clark, J. Horwitz, H. W. Hepburne-Scott, W. W. de Jong, M. J. Crabbe, and J. J. Harding. 2001. Chaperone function of mutant versions of αA- and αB-crystallin prepared to pinpoint chaperone binding sites. Eur. J. Biochem. 268:713-721. [PubMed]
64. Derré, I., G. Rapoport, and T. Msadek. 1999. CtsR, a novel regulator of stress and heat shock response, controls clp and molecular chaperone gene expression in Gram-positive bacteria. Mol. Microbiol. 31:117-131. [PubMed]
65. Derré, I., G. Rapoport, and T. Msadek. 2000. The CtsR regulator of stress response is active as a dimer and specifically degraded in vivo at 37°C. Mol. Microbiol. 38:335-347. [PubMed]
66. Deuerling, E., A. Schulze-Specking, T. Tomoyasu, A. Mogk, and B. Bukau. 1999. Trigger factor and DnaK cooperate in folding of newly synthesized proteins. Nature 400:693-696. [PubMed]
67. Diamant, S., A. P. Ben-Zvi, B. Bukau, and P. Goloubinoff. 2000. Size-dependent disaggregation of stable protein aggregates by the DnaK chaperone machinery. J. Biol. Chem. 275:21107-21113. [PubMed]
68. Downs, C. A., and S. A. Heckathorn. 1998. The mitochondrial small heat-shock protein protects NADH:ubiquinone oxidoreductase of the electron transport chain during heat stress in plants. FEBS Lett. 430:246-250. [PubMed]
69. Downs, C. A., L. R. Jones, and S. A. Heckathorn. 1999. Evidence for a novel set of small heat-shock proteins that associates with the mitochondria of murine PC12 cells and protects NADH:ubiquinone oxidoreductase from heat and oxidative stress. Arch. Biochem. Biophys. 365:344-350. [PubMed]
70. Dukan, S., A. Farewell, M. Ballesteros, F. Taddei, M. Radman, and T. Nyström. 2000. Protein oxidation in response to increased transcriptional or translational errors. Proc. Natl. Acad. Sci. USA 97:5746-5749. [PubMed]
71. Ehrnsperger, M., J. Buchner, and M. Gaestel. 1998. Structure and function of small heat-shock proteins, p. 533-575. In A. L. Fink, and Y. Goto (ed.), Molecular chaperones in the life cycle of proteins: structure, function and mode of action. Marcel Dekker, Inc., New York, N.Y.
72. Ehrnsperger, M., S. Gräber, M. Gaestel, and J. Buchner. 1997. Binding of non-native protein to Hsp25 during heat shock creates a reservoir of folding intermediates for reactivation. EMBO J. 16:221-229. [PubMed]
73. Ehrnsperger, M., C. Hergersberg, U. Wienhues, A. Nichtl, and J. Buchner. 1998. Stabilization of proteins and peptides in diagnostic immunological assays by the molecular chaperone Hsp25. Anal. Biochem. 259:218-225. [PubMed]
74. Ehrnsperger, M., H. Lilie, M. Gaestel, and J. Buchner. 1999. The dynamics of Hsp25 quaternary structure—structure and function of different oligomeric species. J. Biol. Chem. 274:14867-14874. [PubMed]
75. Ellis, J. 1987. Proteins as molecular chaperones. Nature 328:378-379. [PubMed]
76. Ellis, R. J. 1990. The molecular chaperone concept. Semin. Cell Biol. 1:1-9. [PubMed]
77. Ewalt, K. L., J. P. Hendrick, W. A. Houry, and F. U. Hartl. 1997. In vivo observation of polypeptide flux through the bacterial chaperonin system. Cell 90:491-500. [PubMed]
78. Farnsworth, P. N., H. Frauwirth, B. Groth Vasselli, and K. Singh. 1998. Refinement of 3D structure of bovine lens αA-crystallin. Int. J. Biol. Macromol. 22:175-185. [PubMed]
79. Farnsworth, P. N., and K. Singh. 2000. Self-complementary motifs (SCM) in α-crystallin small heat shock proteins. FEBS Lett. 482:175-179. [PubMed]
80. Fayet, O., T. Ziegelhofer, and C. Georgopoulos. 1989. The groES and groEL heat shock gene products of Escherichia coli are essential for bacterial growth at all temperatures. J. Bacteriol. 171:1379-1385. [PMC free article] [PubMed]
81. Feil, I. K., M. Malfois, J. Hendle, H. van der Zandt, and D. I. Svergun. 2001. A novel quaternary structure of the dimeric α-crystallin domain with chaperone-like activity. J. Biol. Chem. 276:12024-12024. [PubMed]
82. Fernando, P., and J. J. Heikkila. 2000. Functional characterization of Xenopus small heat shock protein, Hsp30C: the carboxyl end is required for stability and chaperone activity. Cell Stress Chaperone 5:148-159. [PMC free article] [PubMed]
83. Fischer, H. M., M. Babst, T. Kaspar, G. Acuña, F. Arigoni, and H. Hennecke. 1993. One member of a groESL-like chaperonin multigene family in Bradyrhizobium japonicum is co-regulated with symbiotic nitrogen fixation genes. EMBO J. 12:2901-2912. [PubMed]
84. Fischer, H. M., K. Schneider, M. Babst, and H. Hennecke. 1999. GroEL chaperonins are required for the formation of a functional nitrogenase in Bradyrhizobium japonicum. Arch. Microbiol. 171:279-289.
85. Flaherty, K. M., C. DeLuca-Flaherty, and D. B. McKay. 1990. Three-dimensional structure of the ATPase fragment of a 70K heat-shock cognate protein. Nature 346:623-628. [PubMed]
86. Fleischmann, R. D., M. D. Adams, O. White, R. A. Clayton, E. F. Kirkness, et al. 1995. Whole-genome random sequencing and assembly of Haemophilus influenzae Rd. Science 269:496-512. [PubMed]
87. Fraser, C. M., S. Casjens, W. M. Huang, G. G. Sutton, R. Clayton, et al. 1997. Genomic sequence of a Lyme disease spirochaete, Borrelia burgdorferi. Nature 390:580-586. [PubMed]
88. Fraser, C. M., J. D. Gocayne, O. White, M. D. Adams, R. A. Clayton, et al. 1995. The minimal gene complement of Mycoplasma genitalium. Science 270:397-403. [PubMed]
89. Fraser, C. M., S. J. Norris, G. M. Weinstock, O. White, G. G. Sutton, et al. 1998. Complete genome sequence of Treponema pallidum, the syphilis spirochete. Science 281:375-388. [PubMed]
89a. Galibert, F., T. M. Finan, S. R. Long, A. Pühler, P. Abola, et al. 2001. The composite genome of the legume symbiont Sinorhizobium meliloti. Science 293:668-672. [PubMed]
90. Georgellis, D., B. Sohlberg, F. U. Hartl, and A. von Gabain. 1995. Identification of GroEL as a constituent of an mRNA-protection complex in Escherichia coli. Mol. Microbiol. 16:1259-1268. [PubMed]
91. Glass, J. I., E. J. Lefkowitz, J. S. Glass, C. R. Heiner, E. Y. Chen, and G. H. Cassell. 2000. The complete sequence of the mucosal pathogen Ureaplasma urealyticum. Nature 407:757-762. [PubMed]
92. Glover, J. R., and S. Lindquist. 1998. Hsp104, Hsp70, and Hsp40: A novel chaperone system that rescues previously aggregated proteins. Cell 94:73-82. [PubMed]
93. Goffeau, A., et al. 1997. The yeast genome directory. Nature 387(Suppl.):1-107.
94. Goloubinoff, P., A. Mogk, A. Peres Ben-Zvi, T. Tomoyasu, and B. Bukau. 1999. Sequential mechanism of solubilization and refolding of stable protein aggregates by a bichaperone network. Proc. Natl. Acad. Sci. USA 96:13732-13737. [PubMed]
95. González-Márquez, H., C. Perrin, P. Bracquart, C. Guimont, and G. Linden. 1997. A 16 kDa protein family overexpressed by Streptococcus thermophilus PB18 in acid environments. Microbiology 5:1587-1594. [PubMed]
96. Gottesman, S. 1996. Proteases and their targets in Escherichia coli. Annu. Rev. Genet. 30:465-506. [PubMed]
97. Gottesman, S., S. Wickner, and M. R. Maurizi. 1997. Protein quality control: triage by chaperones and proteases. Genes Dev. 11:815-823. [PubMed]
98. Graumann, P. L., and M. A. Marahiel. 1998. A superfamily of proteins that contain the cold-shock domain. Trends Biochem. Sci. 23:286-290. [PubMed]
 99. Gribaldo, S., V. Lumia, R. Creti, E. C. de Macario, A. Sanangelantoni, and P. Cammarano. 1999. Discontinuous occurrence of the hsp70 (dnaK) gene among Archaea and sequence features of HSP70 suggest a novel outlook on phylogenies inferred from this protein. J. Bacteriol. 181:434-443. [PMC free article] [PubMed]
100. Grimaud, R., M. Kessel, F. Beuron, A. C. Steven, and M. R. Maurizi. 1998. Enzymatic and structural similarities between the Escherichia coli ATP-dependent proteases, ClpXP and ClpAP. J. Biol. Chem. 273:12476-12481. [PubMed]
101. Groenen, P. J. T. A., K. B. Merck, W. W. de Jong, and H. Bloemendal. 1994. Structure and modifications of the junior chaperone α-crystallin: from lens transparency to molecular pathology. Eur. J. Biochem. 225:1-19. [PubMed]
102. Gross, C. A. 1996. Function and regulation of the heat shock proteins, p. 1382-1399. In F. C. Neidhardt et al. (ed.), Escherichia coli and Salmonella: cellular and molecular biology, and ed. American Society for Microbiology, Washington, D.C.
103. Gross, C. A., M. Lonetto, and R. Losick. 1992. Bacterial sigma factors, p. 129-176. In S. L. McKnight and K. R. Yamamoto (ed.), Transcriptional regulation, vol. 1. Cold Spring Harbor Laboratory Press, Cold Spring Harbor, N.Y.
104. Gu, J., M. Emerman, and S. Sandmeyer. 1997. Small heat shock protein suppression of Vpr-induced cytoskeletal defects in budding yeast. Mol. Cell. Biol. 17:4033-4042. [PMC free article] [PubMed]
105. Guglielmi, G., P. Mazodier, C. J. Thompson, and J. Davies. 1991. A survey of the heat shock response in four Streptomyces species reveals two groEL-like genes and three GroEL-like proteins in Streptomyces albus. J. Bacteriol. 173:7374-7381. [PMC free article] [PubMed]
106. Guzzo, J., F. Delmas, F. Pierre, M. P. Jobin, B. Samyn, J. Van Beeumen, J. F. Cavin, and C. Diviès. 1997. A small heat shock protein from Leuconostoc oenos induced by multiple stresses and during stationary growth phase. Lett. Appl. Microbiol. 24:393-396. [PubMed]
107. Haley, D. A., M. P. Bova, Q. L. Huang, H. S. Mchaourab, and P. L. Stewart. 2000. Small heat-shock protein structures reveal a continuum from symmetric to variable assemblies. J. Mol. Biol. 298:261-272. [PubMed]
108. Haley, D. A., J. Horwitz, and P. L. Stewart. 1998. The small heat-shock protein, αB-crystallin, has a variable quaternary structure. J. Mol. Biol. 277:27-35. [PubMed]
109. Harndahl, U., R. B. Hall, K. W. Osteryoung, E. Vierling, J. F. Bornman, and C. Sundby. 1999. The chloroplast small heat shock protein undergoes oxidation-dependent conformational changes and may protect plants from oxidative stress. Cell Stress Chaperones 4:129-138. [PMC free article] [PubMed]
110. Harrison, C. J., M. Hayer-Hartl, M. Di Liberto, F. U. Hartl, and J. Kuriyan. 1997. Crystal structure of the nucleotide exchange factor GrpE bound to the ATPase domain of the molecular chaperone DnaK. Science 276:431-435. [PubMed]
111. Hartl, F. U. 1996. Molecular chaperones in cellular protein folding. Nature 381:571-580. [PubMed]
112. Haslbeck, M., S. Walke, T. Stromer, M. Ehrnsperger, H. E. White, S. X. Chen, H. R. Saibil, and J. Buchner. 1999. Hsp26: a temperature-regulated chaperone. EMBO J. 18:6744-6751. [PubMed]
113. Heckathorn, S. A., C. A. Downs, T. D. Sharkey, and J. S. Coleman. 1998. The small, methionine-rich chloroplast heat-shock protein protects photosystem II electron transport during heat stress. Plant Physiol. 116:439-444. [PubMed]
114. Hecker, M., W. Schumann, and U. Völker. 1996. Heat-shock and general stress response in Bacillus subtilis. Mol. Microbiol. 19:417-428. [PubMed]
115. Heidelbach, M., H. Skladny, and H. U. Schairer. 1993. Heat shock and development induce synthesis of a low-molecular-weight stress-responsive protein in the myxobacterium Stigmatella aurantiaca. J. Bacteriol. 175:7479-7482. [PMC free article] [PubMed]
116. Heidelbach, M., H. Skladny, and H. U. Schairer. 1993. Purification and characterization of SP21, a development-specific protein of the myxobacterium Stigmatella aurantiaca. J. Bacteriol. 175:905-908. [PMC free article] [PubMed]
117. Heidelberg, J. F., J. A. Eisen, W. C. Nelson, R. A. Clayton, M. L. Gwinn, et al. 2000. DNA sequence of both chromosomes of the cholera pathogen Vibrio cholerae. Nature 406:477-483. [PubMed]
118. Heikkila, J. J., N. Ohan, Y. Tam, and A. Ali. 1997. Heat shock protein gene expression during Xenopus development. Cell. Mol. Life Sci. 53:114-121. [PubMed]
119. Helm, K. W., G. J. Lee, and E. Vierling. 1997. Expression and native structure of cytosolic class II small heat shock proteins. Plant Physiol. 114:1477-1485. [PubMed]
120. Henriques, A. O., B. W. Beall, and C. P. Moran. 1997. CotM of Bacillus subtilis, a member of the α-crystallin family of stress proteins, is induced during development and participates in spore outer coat formation. J. Bacteriol. 179:1887-1897. [PMC free article] [PubMed]
121. Herman, C., and R. D'Ari. 1998. Proteolysis and chaperones: the destruction/reconstruction dilemma. Curr. Opin. Microbiol. 1:204-209. [PubMed]
122. Herman, C., D. Thévenet, R. D'Ari, and P. Bouloc. 1995. Degradation of σ32, the heat shock regulator in Escherichia coli, is governed by Hf1B. Proc. Natl. Acad. Sci. USA 92:3516-3520. [PubMed]
123. Hesterkamp, T., and B. Bukau. 1998. Role of the DnaK and HscA homologs of Hsp70 chaperones in protein folding in E. coli. EMBO J. 17:4818-4828. [PubMed]
124. Himmelreich, R., H. Hilbert, H. Plagens, E. Pirkl, B. C. Li, and R. Herrmann. 1996. Complete sequence analysis of the genome of the bacterium Mycoplasma pneumoniae. Nucleic Acids Res. 24:4420-4449. [PMC free article] [PubMed]
125. Horváth, I., A. Glatz, V. Varvasovszki, Z. Török, T. Páli, G. Balogh, E. Kovács, L. Nádasdi, S. Benkö, F. Joó, and L. Vigh. 1998. Membrane physical state controls the signaling mechanism of the heat shock response in Synechocystis PCC 6803: identification of hsp17 as a “fluidity gene.” Proc. Natl. Acad. Sci. USA 95:3513-3518. [PubMed]
126. Horwich, A. L., E. U. Weber-Ban, and D. Finley. 1999. Chaperone rings in protein folding and degradation. Proc. Natl. Acad. Sci. USA 96:11033-11040. [PubMed]
127. Horwitz, J. 1992. α-crystallin can function as a molecular chaperone. Proc. Natl. Acad. Sci. USA 89:10449-10453. [PubMed]
128. Horwitz, J., M. Bova, Q. L. Huang, L. Ding, O. Yaron, and S. Lowman. 1998. Mutation of αB-crystallin: effects on chaperone-like activity. Int. J. Biol. Macromol. 22:263-269. [PubMed]
129. Horwitz, J., M. P. Bova, L. L. Ding, D. A. Haley, and P. L. Stewart. 1999. Lens α-crystallins: function and structure. Eye 13:403-408. [PubMed]
130. Houry, W. A., D. Frishman, C. Eckerskorn, F. Lottspeich, and F. U. Hartl. 1999. Identification of in vivo substrates of the chaperonin GroEL. Nature 402:147-154. [PubMed]
131. Hunt, J. F., A. J. Weaver, S. J. Landry, L. Gierasch, and J. Deisenhofer. 1996. The crystal structure of the GroES co-chaperonin at 2.8 angstrom resolution. Nature 379:37-45. [PubMed]
132. Hwang, B. J., W. J. Park, C. H. Chung, and A. L. Goldberg. 1987. Escherichia coli contains a soluble ATP-dependent protease (Ti) distinct from protease La. Proc. Natl. Acad. Sci. USA 84:5550-5554. [PubMed]
133. Ingolia, T. D., and E. A. Craig. 1982. Four small Drosophila heat shock proteins are related to each other and to mammalian α-crystallin. Proc. Natl. Acad. Sci. USA 79:2360-2364. [PubMed]
134. Ishihama, A. 1993. Protein-protein communication within the transcription apparatus. J. Bacteriol. 175:2483-2489. [PMC free article] [PubMed]
135. Ishikawa, T., F. Beuron, M. Kessel, S. Wickner, M. R. Maurizi, and A. C. Steven. 2001. Translocation pathway of protein substrates in ClpAP protease. Proc. Natl. Acad. Sci. USA 98:4328-4333. [PubMed]
136. Ito, H., K. Kamei, I. Iwamoto, Y. Inaguma, D. Nohara, and K. Kato. 2001. Phosphorylation-induced change of the oligomerization state of αB-crystallin. J. Biol. Chem. 276:5346-5352. [PubMed]
137. Jakob, U., and J. Buchner. 1994. Assisting spontaneity: the role of Hsp90 and small Hsps as molecular chaperones. Trends Biochem. Sci. 19:205-211. [PubMed]
138. Jakob, U., M. Gaestel, K. Engel, and J. Buchner. 1993. Small heat shock proteins are molecular chaperones. J. Biol. Chem. 268:1517-1520. [PubMed]
139. Jakob, U., H. Lilie, I. Meyer, and J. Buchner. 1995. Transient interaction of Hsp90 with early unfolding intermediates of citrate synthase. Implications for heat shock in vivo. J. Biol. Chem. 270:7288-7294. [PubMed]
140. Jakob, U., W. Muse, M. Eser, and J. C. A. Bardwell. 1999. Chaperone activity with a redox switch. Cell 96:341-352. [PubMed]
141. Jinn, T. L., Y. M. Chen, and C. Y. Lin. 1995. Characterization and physiological function of class I low-molecular-mass, heat-shock protein complex in soybean. Plant Physiol. 108:693-701. [PubMed]
142. Jobin, M. P., F. Delmas, D. Garmyn, C. Diviès, and J. Guzzo. 1997. Molecular characterization of the gene encoding an 18-kilodalton small heat shock protein associated with the membrane of Leuconostoc oenos. Appl. Environ. Microbiol. 63:609-614. [PMC free article] [PubMed]
143. Kaneko, T., Y. Nakamura, S. Sato, E. Asamizu, T. Kato, et al. 2000. Complete genome structure of the nitrogen-fixing symbiotic bacterium Mesorhizobium loti. DNA Res. 7:331-338. [PubMed]
144. Kaneko, T., S. Sato, H. Kotani, A. Tanaka, E. Asamizu, et al. 1996. Sequence analysis of the genome of the unicellular cyanobacterium Synechocystis sp. strain PCC6803. II. Sequence determination of the entire genome and assignment of potential protein-coding regions. DNA Res. 3:109-136. [PubMed]
144a. Kappé, G., P. Verschuure, R. L. A. Philipsen, A. A. Staalduinen, P. van de Boogart, W. C. Boelens, and W. W. de Jong. 2001. Characterization of two novel human small heat shock proteins: protein kinase-related HspB8 and testis-specific HspB9. Biochim. Biophys. Acta 1520:1-6. [PubMed]
145. Kato, K., K. Hasegawa, S. Goto, and Y. Inaguma. 1994. Dissociation as a result of phosphorylation of an aggregated form of the small stress protein, hsp27. J. Biol. Chem. 269:11274-11278. [PubMed]
146. Kato, K., H. Shinohara, S. Goto, Y. Inaguma, R. Morishita, and T. Asano. 1992. Copurification of small heat shock protein with αB-crystallin from human skeletal muscle. J. Biol. Chem. 267:7718-7725. [PubMed]
147. Kawarabayasi, Y., Y. Hino, H. Horikawa, S. Yamazaki, Y. Haikawa, et al. 1999. Complete genome sequence of an aerobic hyper-thermophilic crenarchaeon, Aeropyrum pernix K1. DNA Res. 6:83-101. [PubMed]
148. Kawarabayasi, Y., M. Sawada, H. Horikawa, Y. Haikawa, Y. Hino, et al. 1998. Complete sequence and gene organization of the genome of a hyper-thermophilic archaebacterium, Pyrococcus horikoshii OT3. DNA Res. 5:55-76. [PubMed]
149. Kedersha, N. L., M. Gupta, W. Li, I. Miller, and P. Anderson. 1999. RNA-binding proteins TIA-1 and TIAR link the phosphorylation of eIF-2α to the assembly of mammalian stress granules. J. Cell Biol. 147:1431-1442. [PMC free article] [PubMed]
150. Keiler, K. C., P. R. Waller, and R. T. Sauer. 1996. Role of a peptide tagging system in degradation of proteins synthesized from damaged messenger RNA. Science 271:990-993. [PubMed]
151. Keith, L. M. W., J. E. Partridge, and C. L. Bender. 1999. dnaK and the heat stress response of Pseudomonas syringae pv. glycinea. Mol. Plant-Microbe Interact. 12:563-574. [PubMed]
152. Kessel, M., M. R. Maurizi, B. Kim, E. Kocsis, B. L. Trus, S. K. Singh, and A. C. Steven. 1995. Homology in structural organization between ClpAP protease and the eukaryotic 26 S proteasome. J. Mol. Biol. 250:587-594. [PubMed]
153. Kim, K. I., G. W. Cheong, S. C. Park, J. S. Ha, K. M. Woo, S. J. Choi, and C. H. Chung. 2000. Heptameric ring structure of the heat-shock protein ClpB, a protein-activated ATPase in Escherichia coli. J. Mol. Biol. 303:655-666. [PubMed]
154. Kim, K. I., S. C. Park, S. H. Kang, G. W. Cheong, and C. H. Chung. 1999. Selective degradation of unfolded proteins by the self-compartmentalizing HtrA protease, a periplasmic heat shock protein in Escherichia coli. J. Mol. Biol. 294:1363-1374. [PubMed]
155. Kim, K. K., R. Kim, and S. H. Kim 1998. Crystal structure of a small heat-shock protein. Nature 394:595-599. [PubMed]
156. Kim, R., K. K. Kim, H. Yokota, and S. H. Kim. 1998. Small heat shock protein of Methanococcus jannaschii, a hyperthermophile. Proc. Natl. Acad. Sci. USA 95:9129-9133. [PubMed]
156a. Kim, S. J., D. G. Jeong, S. W. Chi, J. S. Lee, and S. E. Ryu. 2001. Crystal structure of proteolytic fragments of the redox-sensitive Hsp33 with constitutive chaperone activity. Nat. Struct. Biol. 8:459-466. [PubMed]
157. Kirschner, M., S. Winkelhaus, J. M. Thierfelder, and L. Nover. 2000. Transient expression and heat-stress-induced co-aggregation of endogenous and heterologous small heat-stress proteins in tobacco protoplasts. Plant J. 24:397-411. [PubMed]
158. Kitagawa, M., Y. Matsumura, and T. Tsuchido. 2000. Small heat shock proteins, IbpA and IbpB, are involved in resistances to heat and superoxide stresses in Escherichia coli. FEMS Microbiol. Lett. 184:165-171. [PubMed]
159. Klenk, H. P., R. A. Clayton, J. F. Tomb, O. White, K. E. Nelson, et al. 1997. The complete genome sequence of the hyperthermophilic, sulphate-reducing archaeon Archaeoglobus fulgidus. Nature 390:364-370. [PubMed]
160. Kokke, B. P. A., M. R. Leroux, E. P. M. Candido, W. C. Boelens, and W. W. de Jong. 1998. Caenorhabditis elegans small heat-shock proteins Hsp12.2 and Hsp12.3 form tetramers and have no chaperone-like activity. FEBS Lett. 433:228-232. [PubMed]
161. Korber, P., J. M. Stahl, K. H. Nierhaus, and J. C. A. Bardwell. 2000. Hsp15: a ribosome-associated heat shock protein. EMBO J. 19:741-748. [PubMed]
162. Koteiche, H. A., and H. S. Mchaourab. 1999. Folding pattern of the α-crystallin domain in αA-crystallin determined by site-directed spin labeling. J. Mol. Biol. 294:561-577. [PubMed]
163. Krüger, E., and M. Hecker. 1998. The first gene of the Bacillus subtilis clpC operon,ctsR, encodes a negative regulator of its own operon and other class III heat shock genes. J. Bacteriol. 180:6681-6688. [PMC free article] [PubMed]
164. Krüger, E., D. Zühlke, E. Witt, H. Ludwig, and M. Hecker. 2001. Clp-mediated proteolysis in Gram-positive bacteria is autoregulated by the stability of a repressor. EMBO J. 20:852-863. [PubMed]
164a. Kuczynska-Wisnik, D., E. Laskowska, and A. Taylor. 2001. Transcription of ibpB heat shock gene is under control of σ32- and σ54-promoters, a third regulon of heat-shock response. Biochem. Biophys. Res. Commun. 284:57-64. [PubMed]
165. Kudva, Y. C., H. J. Hiddinga, P. C. Butler, C. S. Mueske, and N. L. Eberhardt. 1997. Small heat shock proteins inhibit in vitro Aβ1-42 amyloidogenesis. FEBS Lett. 416:117-121. [PubMed]
166. Kumar, L. V., T. Ramakrishna, and C. M. Rao. 1999. Structural and functional consequences of the mutation of a conserved arginine residue in αA and αB crystallins. J. Biol. Chem. 274:24137-24141. [PubMed]
167. Kunst, F., N. Ogasawara, I. Moszer, A. M. Albertini, G. Alloni, et al. 1997. The complete genome sequence of the Gram-positive bacterium Bacillus subtilis. Nature 390:249-256. [PubMed]
168. Lambert, H., S. J. Charette, A. F. Bernier, A. Guimond, and J. Landry. 1999. HSP27 multimerization mediated by phosphorylation-sensitive intermolecular interactions at the amino terminus. J. Biol. Chem. 274:9378-9385. [PubMed]
169. Landry, J., P. Chretien, H. Lambert, E. Hickey, and L. A. Weber. 1989. Heat shock resistance conferred by expression of the human HSP27 gene in rodent cells. J. Cell Biol. 109:7-15. [PMC free article] [PubMed]
170. Laskowska, E., A. Wawrzynów, and A. Taylor. 1996. IbpA and IbpB, the new heat-shock proteins, bind to endogenous Escherichia coli proteins aggregated intracellularly by heat shock. Biochimie 78:117-122. [PubMed]
171. Lavoie, J. N., G. Gingras-Breton, R. M. Tanguay, and J. Landry. 1993. Induction of Chinese hamster HSP27 gene expression in mouse cells confers resistance to heat shock. HSP27 stabilization of the microfilament organization. J. Biol. Chem. 268:3420-3429. [PubMed]
172. Lavoie, J. N., H. Lambert, E. Hickey, L. A. Weber, and J. Landry. 1995. Modulation of cellular thermoresistance and actin filament stability accompanies phosphorylation-induced changes in the oligomeric structure of heat shock protein 27. Mol. Cell. Biol. 15:505-516. [PMC free article] [PubMed]
173. Lee, B. Y., S. A. Hefta, and P. J. Brennan. 1992. Characterization of the major membrane protein of virulent Mycobacterium tuberculosis. Infect. Immun. 60:2066-2074. [PMC free article] [PubMed]
174. Lee, G. J., N. Pokala, and E. Vierling. 1995. Structure and in vitro molecular chaperone activity of cytosolic small heat shock proteins from pea. J. Biol. Chem. 270:10432-10438. [PubMed]
175. Lee, G. J., A. M. Roseman, H. R. Saibil, and E. Vierling. 1997. A small heat shock protein stably binds heat denatured model substrates and can maintain a substrate in a folding competent state. EMBO J. 16:659-671. [PubMed]
176. Lee, G. J., and E. Vierling. 2000. A small heat shock protein cooperates with heat shock protein 70 systems to reactivate a heat-denatured protein. Plant Physiol. 122:189-197. [PubMed]
177. Lee, S., H. A. Owen, D. J. Prochaska, and S. R. Barnum. 2000. HSP16.6 is involved in the development of thermotolerance and thylakoid stability in the unicellular cyanobacterium, Synechocystis sp. PCC 6803. Curr. Microbiol. 40:283-287. [PubMed]
178. Lee, S. Y., D. J. Prochaska, F. Fang, and S. R. Barnum. 1998. A 16.6-kilodalton protein in the cyanobacterium Synechocystis sp. PCC 6803 plays a role in the heat shock response. Curr. Microbiol. 37:403-407. [PubMed]
179. Leigh, J. A. 1999. Transcriptional regulation in Archaea. Curr. Opin. Microbiol. 2:131-134. [PubMed]
180. Leonhard, K., A. Stiegler, W. Neupert, and T. Langer. 1999. Chaperone-like activity of the AAA domain of the yeast Yme1 AAA protease. Nature 398:348-351. [PubMed]
181. Leroux, M. R., B. J. Ma, G. Batelier, R. Melki, and E. P. M. Candido. 1997. Unique structural features of a novel class of small heat shock proteins. J. Biol. Chem. 272:12847-12853. [PubMed]
182. Leroux, M. R., R. Melki, B. Gordon, G. Batelier, and E. P. M. Candido. 1997. Structure-function studies on small heat shock protein oligomeric assembly and interaction with unfolded polypeptides. J. Biol. Chem. 272:24646-24656. [PubMed]
183. Li, M., and S. L. Wong 1992. Cloning and characterization of the groESL operon from Bacillus subtilis. J. Bacteriol. 174:3981-3992. [PMC free article] [PubMed]
184. Liang, P., and T. H. MacRae. 1997. Molecular chaperones and the cytoskeleton. J. Cell Sci. 110:1431-1440. [PubMed]
185. Linder, B., Z. Jin, J. H. Freedman, and C. S. Rubin. 1996. Molecular characterization of a novel, developmentally regulated small embryonic chaperone from Caenorhabditis elegans. J. Biol. Chem. 271:30158-30166. [PubMed]
186. Lindner, R. A., J. A. Carver, M. Ehrnsperger, J. Buchner, G. Esposito, J. Behlke, G. Lutsch, A. Kotlyarov, and M. Gaestel. 2000. Mouse Hsp25, a small heat shock protein—the role of its C-terminal extension in oligomerization and chaperone action. Eur. J. Biochem. 267:1923-1932. [PubMed]
187. Lindner, R. A., A. Kapur, and J. A. Carver. 1997. The interaction of the molecular chaperone, α-crystallin, with molten globule states of bovine α-lactalbumin. J. Biol. Chem. 272:27722-27729. [PubMed]
188. Lindner, R. A., A. Kapur, M. Mariani, S. J. Titmuss, and J. A. Carver. 1998. Structural alterations of α-crystallin during its chaperone action. Eur. J. Biochem. 258:170-183. [PubMed]
189. Lindquist, S., and E. A. Craig 1988. The heat-shock proteins. Annu. Rev. Genet. 22:631-677. [PubMed]
190. Liu, C., and M. J. Welsh. 1999. Identification of a site of Hsp27 binding with Hsp27 and αB-crystallin as indicated by the yeast two-hybrid system. Biochem. Biophys. Res. Commun. 255:256-261. [PubMed]
191. Lünsdorf, H., H. U. Schairer, and M. Heidelbach. 1995. Localization of the stress protein SP21 in indole-induced spores, fruiting bodies, and heat-shocked cells of Stigmatella aurantiaca. J. Bacteriol. 177:7092-7099. [PMC free article] [PubMed]
191a. Lund, A. A., D. M. Rhoads, A. L. Lund, R. L. Cerny, and T. E. Elthon. 2001. In vivo modifications of the maize mitochondrial small heat stress protein, HSP22. J. Biol. Chem. 276:29924-29929. [PubMed]
192. Macario, A. J., and E. Conway de Macario. 2001. The molecular chaperone system and other anti-stress mechanisms in archaea. Frontiers Biosci. 6:262-283. [PubMed]
192a. Macario, A. J. L., M. Lange, B. K. Ahring, and E. Conway de Macario. 1999. Stress genes and proteins in the archaea. Microbiol. Mol. Biol. Rev. 63:923-967. [PMC free article] [PubMed]
193. MacRae, T. H. 2000. Structure and function of small heat shock/α-crystallin proteins: established concepts and emerging ideas. Cell. Mol. Life Sci. 57:899-913. [PubMed]
194. Manabe, Y. C., J. M. Chen, C. G. Ko, P. Chen, and W. R. Bishai. 1999. Conditional sigma factor expression, using the inducible acetamidase promoter, reveals that the Mycobacterium tuberculosis sigF gene modulates expression of the 16-kilodalton α-crystallin homologue. J. Bacteriol. 181:7629-7633. [PMC free article] [PubMed]
195. Manna, A. C., and H. K. Das. 1997. Characterization and mutagenesis of the leucine biosynthetic genes of Azotobacter vinelandii: an analysis of the rarity of amino acid auxotrophs. Mol. Gen. Genet. 254:207-217. [PubMed]
196. Mayer, M. P., S. Rüdiger, and B. Bukau. 2000. Molecular basis for interactions of the DnaK chaperone with substrates. Biol. Chem. 381:877-885. [PubMed]
197. McDuffee, A. T., G. Senisterra, S. Huntley, J. R. Lepock, K. R. Sekhar, M. J. Meredith, M. J. Borrelli, J. D. Morrow, and M. L. Freeman. 1997. Proteins containing non-native disulfide bonds generated by oxidative stress can act as signals for the induction of the heat shock response. J. Cell. Physiol. 171:143-151. [PubMed]
198. Mehlen, P., J. Briolay, L. Smith, C. Diaz-latoud, N. Fabre, D. Pauli, and A. P. Arrigo. 1993. Analysis of the resistance to heat and hydrogen peroxide stresses in COS cells transiently expressing wild type or deletion mutants of the Drosophila 27-kDa heat-shock protein. Eur. J. Biochem. 215:277-284. [PubMed]
199. Mehlen, P., C. Kretz-Remy, X. Preville, and A. P. Arrigo. 1996. Human hsp27,Drosophila hsp27 and human alphaB-crystallin expression-mediated increase in glutathione is essential for the protective activity of these proteins against TNF α-induced cell death. EMBO J. 15:2695-2706. [PubMed]
200. Mehlen, P., A. Mehlen, J. Godet, and A. P. Arrigo. 1997. hsp27 as a switch between differentiation and apoptosis in murine embryonic stem cells. J. Biol. Chem. 272:31657-31665. [PubMed]
201. Mehlen, P., K. Schulze-Osthoff, and A. P. Arrigo. 1996. Small stress proteins as novel regulators of apoptosis. Heat shock protein 27 blocks Fas/APO-1- and staurosporine-induced cell death. J. Biol. Chem. 271:16510-16514. [PubMed]
202. Merck, K. B., P. J. T. A. Groenen, C. E. M. Voorter, W. A. de Haard-Hoekman, J. Horwitz, H. Bloemendal, and W. W. de Jong. 1993. Structural and functional similarities of bovine α-crystallin and mouse small heat-shock protein — a family of chaperones. J. Biol. Chem. 268:1046-1052. [PubMed]
203. Michaud, S., R. Marin, and R. M. Tanguay. 1997. Regulation of heat shock gene induction and expression during Drosophila development. Cell. Mol. Life Sci. 53:104-113. [PubMed]
204. Michelini, E. T., and G. C. Flynn. 1999. The unique chaperone operon of Thermotoga maritima: cloning and initial characterization of a functional Hsp70 and small heat shock protein. J. Bacteriol. 181:4237-4244. [PMC free article] [PubMed]
205. Michiels, J., C. Verreth, and J. Vanderleyden. 1994. Effects of temperature stress on bean-nodulating Rhizobium strains. Appl. Environ. Microbiol. 60:1206-1212. [PMC free article] [PubMed]
206. Minder, A. C., F. Narberhaus, M. Babst, H. Hennecke, and H. M. Fischer. 1997. The dnaKJ operon belongs to the σ32 dependent class of heat shock genes in Bradyrhizobium japonicum. Mol. Gen. Genet. 254:195-206. [PubMed]
207. Miron, T., K. Vancompernolle, J. Vandekerckhove, M. Wilchek, and B. Geiger. 1991. A 25-kD inhibitor of actin polymerization is a low molecular mass heat shock protein. J. Cell Biol. 114:255-261. [PMC free article] [PubMed]
208. Missiakas, D., and S. Raina. 1998. The extracytoplamic function sigma factors: role and regulation. Mol. Microbiol. 28:1059-1066. [PubMed]
209. Missiakas, D., F. Schwager, J. M. Betton, C. Georgopoulos, and S. Raina. 1996. Identification and characterization of HslV HslU (ClpQ ClpY) proteins involved in overall proteolysis of misfolded proteins in Escherichia coli. EMBO J. 15:6899-6909. [PubMed]
210. Mogk, A., G. Homuth, C. Scholz, L. Kim, F. X. Schmid, and W. Schumann. 1997. The GroE chaperonin machine is a major modulator of the CIRCE heat shock regulon of Bacillus subtilis. EMBO J. 16:4579-4590. [PubMed]
211. Mogk, A., T. Tomoyasu, P. Goloubinoff, S. Rüdiger, D. Röder, H. Langen, and B. Bukau. 1999. Identification of thermolabile Escherichia coli proteins: prevention and reversion of aggregation by DnaK and ClpB. EMBO J. 18:6934-6949. [PubMed]
212. Morimoto, R. I. 1998. Regulation of the heat shock transcriptional response: cross talk between a family of heat shock factors, molecular chaperones, and negative regulators. Genes Dev. 12:3788-3796. [PubMed]
213. Morimoto, R. I., A. Tissières, and C. Georgopoulos. 1994. Progress and perspectives on the biology of heat shock proteins and molecular chaperones, p. 1-30. In R. I. Morimoto, A. Tissières, and C. Georgopoulos (ed.), The biology of heat shock proteins and molecular chaperones. Cold Spring Harbor Laboratory Press, Cold Spring Harbor, N.Y.
214. Motohashi, K., Y. Watanabe, M. Yohda, and M. Yoshida. 1999. Heat-inactivated proteins are rescued by the DnaKJ-GrpE set and ClpB chaperones. Proc. Natl. Acad. Sci. USA 96:7184-7189. [PubMed]
215. Muchowski, P. J., J. A. Bassuk, N. H. Lubsen, and J. I. Clark. 1997. Human αB crystallin: small heat shock protein and molecular chaperone. J. Biol. Chem. 272:2578-2582. [PubMed]
216. Muchowski, P. J., and J. I. Clark. 1998. ATP-enhanced molecular chaperone functions of the small heat shock protein human αB crystallin. Proc. Natl. Acad. Sci. USA 95:1004-1009. [PubMed]
217. Muchowski, P. J., L. G. Hays, J. R. Yates, and J. I. Clark. 1999. ATP and the core“α-crystallin” domain of the small heat-shock protein αB-crystallin. J. Biol. Chem. 274:30190-30195. [PubMed]
218. Muchowski, P. J., G. J. S. Wu, J. J. N. Liang, E. T. Adman, and J. I. Clark. 1999. Site-directed mutations within the core “α-crystallin” domain of the small heat-shock protein, human αB-crystallin, decrease molecular chaperone functions. J. Mol. Biol. 289:397-411. [PubMed]
219. Münchbach, M., P. Dainese, W. Staudenmann, F. Narberhaus, and P. James. 1999. Proteome analysis of heat shock protein expression in Bradyrhizobium japonicum. Eur. J. Biochem. 264:39-48. [PubMed]
220. Münchbach, M., A. Nocker, and F. Narberhaus. 1999. Multiple small heat shock proteins in rhizobia. J. Bacteriol. 181:83-90. [PMC free article] [PubMed]
221. Nakamoto, H., N. Suzuki, and S. K. Roy. 2000. Constitutive expression of a small heat-shock protein confers cellular thermotolerance and thermal protection to the photosynthetic apparatus in cyanobacteria. FEBS Lett. 483:169-174. [PubMed]
222. Narberhaus, F. 1999. Negative regulation of bacterial heat shock genes. Mol. Microbiol. 31:1-8. [PubMed]
223. Narberhaus, F., R. Käser, A. Nocker, and H. Hennecke. 1998. A novel DNA element that controls bacterial heat shock gene expression. Mol. Microbiol. 28:315-323. [PubMed]
224. Narberhaus, F., W. Weiglhofer, H. M. Fischer, and H. Hennecke. 1996. The Bradyrhizobium japonicum rpoH1 gene encoding a σ32-like protein is part of a unique heat shock gene cluster together with groESL1 and three small heat shock genes. J. Bacteriol. 178:5337-5346. [PMC free article] [PubMed]
225. Narberhaus, F., W. Weiglhofer, H. M. Fischer, and H. Hennecke. 1998. Identification of the Bradyrhizobium japonicum degP gene as part of an operon containing small heat-shock protein genes. Arch. Microbiol. 169:89-97. [PubMed]
226. Natera, S. H. A., N. Guerreiro, and N. A. Djordjevic. 2000. Proteome analysis of differentially displayed proteins as a tool for the investigation of symbiosis. Mol. Plant-Microbe Interact. 13:995-1009. [PubMed]
227. Nelson, K. E., R. A. Clayton, S. R. Gill, M. L. Gwinn, R. J. Dodson, et al. 1999. Evidence for lateral gene transfer between Archaea and Bacteria from genome sequence of Thermotoga maritima. Nature 399:323-329. [PubMed]
228. Nerland, A. H., A. S. Mustafa, D. Sweetser, T. Godal, and R. A. Young. 1988. A protein antigen of Mycobacterium leprae is related to a family of small heat shock proteins. J. Bacteriol. 170:5919-5921. [PMC free article] [PubMed]
229. Netzer, W. J., and F. U. Hartl. 1998. Protein folding in the cytosol: chaperonin-dependent and -independent mechanisms. Trends Biochem. Sci. 23:68-73. [PubMed]
230. Ng, W. V., S. P. Kennedy, G. G. Mahairas, B. Berquist, M. Pan, et al. 2000. Genome sequence of Halobacterium species NRC-1. Proc. Natl. Acad. Sci. USA 97:12176-12181. [PubMed]
231. Reference deleted.
232. Nicholl, I. D., and R. A. Quinlan. 1994. Chaperone activity of α-crystallins modulates intermediate filament assembly. EMBO J. 13:945-953. [PubMed]
233. Nierman, W. C., T. V. Feldblyum, M. T. Laub, I. T. Paulsen, K. E. Nelson, et al. 2001. Complete genome sequence of Caulobacter crescentus. Proc. Natl. Acad. Sci. USA 98:4136-4141. [PubMed]
234. Nocker, A., T. Hausherr, S. Balsiger, N. P. Krstulovic, H. Hennecke, and F. Narberhaus. 2001. A mRNA-based thermosensor controls expression of rhizobial heat shock genes. Nucleic Acids Res. 29:4800-4807. [PMC free article] [PubMed]
235. Nocker, A., N. P. Krstulovic, X. Perret, and F. Narberhaus. 2001. ROSE elements occur in disparate rhizobia and are functionally interchangeable between species. Arch. Microbiol. 176:44-51. [PubMed]
235a. Nölling, J., G. Breton, M. V. Omelchenko, K. S. Makarova, Q. Zeng, et al. 2001. Genome sequence and comparative analysis of the solvent-producing bacterium Clostridium acetobutylicum. J. Bacteriol. 183:4823-4838. [PMC free article] [PubMed]
236. Nover, L., and K. D. Scharf. 1997. Heat stress proteins and transcription factors. Cell. Mol. Life Sci. 53:80-103. [PubMed]
237. Nover, L., K. D. Scharf, and D. Neumann. 1989. Cytoplasmic heat shock granules are formed from precursor particles and are associated with a specific set of mRNAs. Mol. Cell. Biol. 9:1298-1308. [PMC free article] [PubMed]
238. Ogawa, J., and S. R. Long. 1995. The Rhizobium meliloti groELc locus is required for regulation of early nod genes by the transcription activator NodD. Genes Dev. 9:714-729. [PubMed]
239. O'Sullivan, T., D. van Sinderen, and G. Fitzgerald. 1999. Structural and functional analysis of pCI65st, a 6.5 kb plasmid from Streptococcus thermophilus NDI-6. Microbiology 145:127-134. [PubMed]
240. Paek, K. H., and G. C. Walker. 1987. Escherichia coli dnaK mutants are inviable at high temperatures. J. Bacteriol. 169:283-290. [PMC free article] [PubMed]
241. Panaretou, B., C. Prodromou, S. M. Roe, R. Obrien, J. E. Ladbury, P. W. Piper, and L. H. Pearl. 1998. ATP binding and hydrolysis are essential to the function of the Hsp90 molecular chaperone in vivo. EMBO J. 17:4829-4836. [PubMed]
242. Parkhill, J., B. W. Wren, K. Mungall, J. M. Ketley, C. Churcher, et al. 2000. The genome sequence of the food-borne pathogen Campylobacter jejuni reveals hypervariable sequences. Nature 403:665-668. [PubMed]
243. Pellecchia, M., T. Szyperski, D. Wall, C. Georgopoulos, and K. Wüthrich. 1996. NMR structure of the J-domain and the Gly/Phe-rich region of the Escherichia coli DnaJ chaperone. J. Mol. Biol. 260:236-250. [PubMed]
244. Perng, M. D., P. J. Muchowski, P. van den Ijssel, G. J. Wu, A. M. Hutcheson, J. I. Clark, and R. A. Quinlan. 1999. The cardiomyopathy and lens cataract mutation inαB-crystallin alters its protein structure, chaperone activity, and interaction with intermediate filaments in vitro. J. Biol. Chem. 274:33235-33243. [PubMed]
245. Pich, A., F. Narberhaus, and H. Bahl. 1990. Induction of heat shock proteins during initiation of solvent formation in Clostridium acetobutylicum. Appl. Microbiol. Biotechnol. 33:697-704.
246. Pietrowski, D., M. J. Durante, A. Liebstein, T. Schmitt-John, T. Werner, and J. Graw. 1994. α-Crystallins are involved in specific interactions with the murine gamma D/E/F-crystallin-encoding gene. Gene 144:171-178. [PubMed]
247. Plater, M. L., D. Goode, and M. J. Crabbe. 1996. Effects of site-directed mutations on the chaperone-like activity of αB-crystallin. J. Biol. Chem. 271:28558-28566. [PubMed]
248. Plesofsky-Vig, N., and R. Brambl. 1995. Disruption of the gene for hsp30, an α-crystallin-related heat shock protein of Neurospora crassa, causes defects in thermotolerance. Proc. Natl. Acad. Sci. USA 92:5032-5036. [PubMed]
249. Rajaraman, K., B. Raman, T. Ramakrishna, and C. M. Rao. 1998. The chaperone-likeα-crystallin forms a complex only with the aggregation-prone molten globule state of α-lactalbumin. Biochem. Biophys. Res. Commun. 249:917-921. [PubMed]
250. Raman, B., and C. M. Rao. 1997. Chaperone-like activity and temperature-induced structural changes of α-crystallin. J. Biol. Chem. 272:23559-23564. [PubMed]
251. Ranson, N. A., H. E. White, and H. R. Saibil. 1998. Chaperonins. Biochem. J. 2:233-242. [PubMed]
252. Read, T. D., R. C. Brunham, C. Shen, S. R. Gill, J. F. Heidelberg, et al. 2000. Genome sequences of Chlamydia trachomatis MoPn and Chlamydia pneumoniae AR39. Nucleic Acids Res. 28:1397-1406. [PMC free article] [PubMed]
253. Reddy, G. B., K. P. Das, J. M. Petrash, and W. K. Surewicz. 2000. Temperature-dependent chaperone activity and structural properties of human αA- and αB-crystallins. J. Biol. Chem. 275:4565-4570. [PubMed]
254. Reid, B. G., W. A. Fenton, A. L. Horwich, and E. U. Weber-Ban. 2001. ClpA mediates directional translocation of substrate proteins into the ClpP protease. Proc. Natl. Acad. Sci. USA 98:3768-3772. [PubMed]
255. Reischl, S., S. Thake, G. Homuth, and W. Schumann. 2001. Transcriptional analysis of three Bacillus subtilis genes coding for proteins with the α-crystallin domain characteristic of small heat shock proteins. FEMS Microbiol. Lett. 194:99-103. [PubMed]
256. Rep, M., J. M. van Dijl, K. Suda, G. Schatz, L. A. Grivell, and C. K. Suzuki. 1996. Promotion of mitochondrial membrane complex assembly by a proteolytically inactive yeast Lon. Science 274:103-106. [PubMed]
257. Richardson, A., S. J. Landry, and C. Georgopoulos. 1998. The ins and outs of a molecular chaperone machine. Trends Biochem. Sci. 23:138-143. [PubMed]
258. Richmond, C. S., J. D. Glasner, R. Mau, H. Jin, and F. R. Blattner. 1999. Genome-wide expression profiling in Escherichia coli K-12. Nucleic Acids Res. 27:3821-3835. [PMC free article] [PubMed]
259. Rogalla, T., M. Ehrnsperger, X. Preville, A. Kotlyarov, G. Lutsch, C. Ducasse, C. Paul, M. Wieske, A. P. Arrigo, J. Buchner, and M. Gaestel. 1999. Regulation of Hsp27 oligomerization, chaperone function, and protective activity against oxidative stress/tumor necrosis factor α by phosphorylation. J. Biol. Chem. 274:18947-18956. [PubMed]
260. Rohrwild, M., O. Coux, H. C. Huang, R. P. Moerschell, S. J. Yoo, J. H. Seol, C. H. Chung, and A. L. Goldberg. 1996. HslV-HslU: A novel ATP-dependent protease complex in Escherichia coli related to the eukaryotic proteasome. Proc. Natl. Acad. Sci. USA 93:5808-5813. [PubMed]
261. Rollet, E., J. N. Lavoie, J. Landry, and R. M. Tanguay. 1992. Expression of Drosophila's 27 kDa heat shock protein into rodent cells confers thermal resistance. Biochem. Biophys. Res. Commun. 185:116-120. [PubMed]
262. Roy, S. K., T. Hiyama, and H. Nakamoto. 1999. Purification and characterization of the 16-kDa heat-shock-responsive protein from the thermophilic cyanobacterium Synechococcus vulcanus, which is an α-crystallin-related, small heat shock protein. Eur. J. Biochem. 262:406-416. [PubMed]
263. Roy, S. K., and H. Nakamoto. 1998. Cloning, characterization, and transcriptional analysis of a gene encoding an α-crystallin-related, small heat shock protein from the thermophilic cyanobacterium Synechococcus vulcanus. J. Bacteriol. 180:3997-4001. [PMC free article] [PubMed]
264. Ruepp, A., W. Graml, M. L. Santos-Martinez, K. K. Koretle, C. Volker, H. W. Mewes, D. Frishman, S. Stocker, A. N. Lupas, and W. Baumeister. 2000. The genome sequence of the thermoacidophilic scavenger Thermoplasma acidophilum. Nature 407:508-513. [PubMed]
265. Sabehat, A., S. Lurie, and D. Weiss. 1998. Expression of small heat-shock proteins at low temperatures. A possible role in protecting against chilling injuries. Plant Physiol. 117:651-658. [PubMed]
266. Sabehat, A., D. Weiss, and S. Lurie. 1996. The correlation between heat-shock protein accumulation and persistence and chilling tolerance in tomato fruit. Plant Physiol. 110:531-537. [PubMed]
266a. Santhoshkumar, P., and K. K. Sharma. 2001. Phe71 is essential for chaperone-like function in αA-crystallin. J. Biol. Chem. 276:47094-47099. [PubMed]
267. Sauer, U., and P. Dürre. 1993. Sequence and molecular characterization of a DNA region encoding a small heat shock protein of Clostridium acetobutylicum. J. Bacteriol. 175:3394-3400. [PMC free article] [PubMed]
268. Scharf, K. D., H. Heider, I. Höhfeld, R. Lyck, E. Schmidt, and L. Nover. 1998. The tomato Hsf system: HsfA2 needs interaction with HsfA1 for efficient nuclear import and may be localized in cytoplasmic heat stress granules. Mol. Cell. Biol. 18:2240-2251. [PMC free article] [PubMed]
268a. Scharf, K. D., M. Siddique, and E. Vierling. 2001. The expanding family of Arabidopsis thaliana small heat stress proteins and a new family of proteins containing α-crystallin domains (Acd proteins). Cell Stress Chaperones 6:225-237. [PMC free article] [PubMed]
269. Schirmer, E. C., J. R. Glover, M. A. Singer, and S. Lindquist. 1996. HSP100/Clp proteins: a common mechanism explains diverse functions. Trends Biochem. Sci. 21:289-296. [PubMed]
270. Schirmer, E. C., S. Lindquist, and E. Vierling. 1994. An Arabidopsis heat shock protein complements a thermotolerance defect in yeast. Plant Cell 6:1899-1909. [PubMed]
271. Schulz, A., B. Tzschaschel, and W. Schumann. 1995. Isolation and analysis of mutants of the dnaK operon of Bacillus subtilis. Mol. Microbiol. 15:421-429. [PubMed]
272. Schumann, W. 1999. FtsH—a single-chain charonin? FEMS Microbiol. Rev. 23:1-11. [PubMed]
273. Seaton, B. L., and L. E. Vickery. 1994. A gene encoding a DnaK/hsp70 homolog in Escherichia coli. Proc. Natl. Acad. Sci. USA 91:2066-2070. [PubMed]
274. Servant, P., C. Grandvalet, and P. Mazodier. 2000. The RheA repressor is the thermosensor of the HSP18 heat shock response of Streptomyces albus. Proc. Natl. Acad. Sci. USA 97:3538-3543. [PubMed]
275. Servant, P., and P. Mazodier. 1995. Characterization of Streptomyces albus 18-kilodalton heat shock-responsive protein. J. Bacteriol. 177:2998-3003. [PMC free article] [PubMed]
276. Servant, P., and P. Mazodier. 1996. Heat induction of hsp18 gene expression in Streptomyces albus G: transcriptional and posttranscriptional regulation. J. Bacteriol. 178:7031-7036. [PMC free article] [PubMed]
277. Servant, P., G. Rapoport, and P. Mazodier. 1999. RheA, the repressor of hsp18 in Streptomyces albus G. Microbiology 9:2385-2391. [PubMed]
278. Sharma, K. K., H. Kaur, and K. Kester. 1997. Functional elements in molecular chaperone α-crystallin: identification of binding sites in αB-crystallin. Biochem. Biophys. Res. Commun. 239:217-222. [PubMed]
279. Sharma, K. K., H. Kaur, G. S. Kumar, and K. Kester. 1998. Interaction of 1,1′-bi(4-anilino)naphthalene-5,5′-disulfonic acid with α-crystallin. J. Biol. Chem. 273:8965-8970. [PubMed]
280. Sharma, K. K., G. S. Kumar, A. S. Murphy, and K. Kester. 1998. Identification of 1,1′-bi(4-anilino)naphthalene-5,5′-disulfonic acid binding sequences in α-crystallin. J. Biol. Chem. 273:15474-15478. [PubMed]
281. Sharma, K. K., R. S. Kumar, G. S. Kumar, and P. T. Quinn. 2000. Synthesis and characterization of a peptide identified as a functional element in αA-crystallin. J. Biol. Chem. 275:3767-3771. [PubMed]
282. Shearstone, J. R., and F. Baneyx. 1999. Biochemical characterization of the small heat shock protein IbpB from Escherichia coli. J. Biol. Chem. 274:9937-9945. [PubMed]
283. Sherman, D. R., M. Voskuil, D. Schnappinger, R. Liao, M. I. Harrell, and G. K. Schoolnik. 2001. Regulation of the Mycobacterium tuberculosis hypoxic response gene encoding α-crystallin. Proc. Natl. Acad. Sci. USA 98:7534-7539. [PubMed]
284. Shi, Y., and R. I. Morimoto. 1999. Autoregulation of the heat shock response. Stress Proteins 136:225-241.
285. Shigenobu, S., H. Watanabe, M. Hattori, Y. Sakaki, and H. Ishikawa. 2000. Genome sequence of the endocellular bacterial symbiont of aphids Buchnera sp. APS. Nature 407:81-86. [PubMed]
286. Shirai, Y., Y. Akiyama, and K. Ito. 1996. Suppression of ftsH mutant phenotypes by overproduction of molecular chaperones. J. Bacteriol. 178:1141-1145. [PMC free article] [PubMed]
287. Shotland, Y., S. Koby, D. Teff, N. Mansur, D. A. Oren, K. Tatematsu, T. Tomoyasu, M. Kessel, B. Bukau, T. Ogura, and A. B. Oppenheim. 1997. Proteolysis of the phage λ CII regulatory protein by FtsH (HflB) of Escherichia coli. Mol. Microbiol. 24:1303-1310. [PubMed]
288. Shroff, N. P., M. Cherian-Shaw, S. Bera, and E. C. Abraham. 2000. Mutation of R116C results in highly oligomerized αA-crystallin with modified structure and defective chaperone-like function. Biochemistry 39:1420-1426. [PubMed]
289. Simpson, A. J. G., F. C. Reinach, P. Arruda, F. A. Abreu, M. Acencio, et al. 2000. The genome sequence of the plant pathogen Xylella fastidiosa. Nature 406:151-157. [PubMed]
290. Singh, K., B. Groth Vasselli, and P. N. Farnsworth. 1998. Interaction of DNA with bovine lens α-crystallin: its functional implications. Int. J. Biol. Macromol. 22:315-320. [PubMed]
291. Singh, S. K., R. Grimaud, J. R. Hoskins, S. Wickner, and M. R. Maurizi. 2000. Unfolding and internalization of proteins by the ATP-dependent proteases ClpXP and ClpAP. Proc. Natl. Acad. Sci. USA 97:8898-903. [PubMed]
292. Smith, D. R., L. A. Doucette-Stamm, C. Deloughery, H. M. Lee, J. Dubois, et al. 1997. Complete genome sequence of Methanobacterium thermoautotrophicum Delta H: functional analysis and comparative genomics. J. Bacteriol. 179:7135-7155. [PMC free article] [PubMed]
293. Smulders, R. H., and W. W. de Jong. 1997. The hydrophobic probe 4,4′-bis(1-anilino-8-naphthalene sulfonic acid) is specifically photoincorporated into the N-terminal domain of αB-crystallin. FEBS Lett. 409:101-104. [PubMed]
294. Smulders, R. H. P. H., J. A. Carver, R. A. Lindner, M. A. M. van Boekel, H. Bloemendal, and W. W. de Jong. 1996. Immobilization of the C-terminal extension of bovine αA-crystallin reduces chaperone-like activity. J. Biol. Chem. 271:29060-29066. [PubMed]
295. Smulders, R. H. P. H., M. A. M. van Boekel, and W. W. de Jong. 1998. Mutations and modifications support a ”pitted-flexiball' model for α-crystallin. Int. J. Biol. Macromol. 22:187-196. [PubMed]
296. Smýkal, P., I. Hrdý, and P. M. Pechan. 2000. High-molecular-mass complexes formed in vivo contain smHSPs and HSP70 and display chaperone-like activity. Eur. J. Biochem. 267:2195-2207. [PubMed]
297. Smýkal, P., J. Masin, I. Hrdý, I. Konopásek, and V. Zárský. 2000. Chaperone activity of tobacco HSP18, a small heat-shock protein, is inhibited by ATP. Plant J. 23:703-713. [PubMed]
298. Solow, B. T., and G. A. Somkuti. 2000. Comparison of low-molecular-weight heat stress proteins encoded on plasmids in different strains of Streptococcus thermophilus. Curr. Microbiol. 41:177-181. [PubMed]
299. Somkuti, G. A., D. K. Y. Solaiman, and D. H. Steinberg. 1998. Structural and functional properties of the hsp16.4-bearing plasmid pER341 in Streptococcus thermophilus. Plasmid 40:61-72. [PubMed]
300. Soppa, J. 1999. Transcription initiation in Archaea: facts, factors and future aspects. Mol. Microbiol. 31:1295-1305. [PubMed]
301. Soto, A., I. Allona, C. Collada, M. A. Guevara, R. Casado, E. Rodriguez-Cerezo, C. Aragoncillo, and L. Gomez. 1999. Heterologous expression of a plant small heat-shock protein enhances Escherichia coli viability under heat and cold stress. Plant Physiol. 120:521-528. [PubMed]
302. Spence, J., and C. Georgopoulos. 1989. Purification and properties of the Escherichia coli heat shock protein, HtpG. J. Biol. Chem. 264:4398-4403. [PubMed]
303. Spiess, C., A. Beil, and M. Ehrmann. 1999. A temperature-dependent switch from chaperone to protease in a widely conserved heat shock protein. Cell 97:339-347. [PubMed]
304. Squires, C., and C. L. Squires. 1992. The Clp proteins: proteolysis regulators or molecular chaperones? J. Bacteriol. 174:1081-1085. [PMC free article] [PubMed]
305. Srinivas, V., S. A. Datta, T. Ramakrishna, and C. M. Rao. 2001. Studies on the α-crystallin target protein sites: sequential binding with two target proteins. Mol. Vis. 7:114-119. [PubMed]
306. Stahlberg, H., E. Kutejova, K. Suda, B. Wolpensinger, A. Lustig, G. Schatz, A. Engel, and C. K. Suzuki. 1999. Mitochondrial Lon of Saccharomyces cerevisiae is a ring-shaped protease with seven flexible subunits. Proc. Natl. Acad. Sci. USA 96:6787-6790. [PubMed]
307. Stege, G. J., K. Renkawek, P. S. Overkamp, P. Verschuure, A. F. van Rijk, A. Reijnen-Aalbers, W. C. Boelens, G. J. Bosman, and W. W. de Jong. 1999. The molecular chaperone αB-crystallin enhances amyloid beta neurotoxicity. Biochem. Biophys. Res. Commun. 262:152-156. [PubMed]
308. Stover, C. K., X. Q. Pham, A. L. Erwin, S. D. Mizoguchi, P. Warrener, et al. 2000. Complete genome sequence of Pseudomonas aeruginosa. PAO1, an opportunistic pathogen. Nature 406:959-964. [PubMed]
309. Reference deleted.
310. Studer, S., and F. Narberhaus. 2000. Chaperone activity and homo- and hetero-oligomer formation of bacterial small heat shock proteins. J. Biol. Chem. 275:37212-37218. [PubMed]
311. Sun, T. X., B. K. Das, and J. J. N. Liang. 1997. Conformational and functional differences between recombinant human lens αA- and αB-crystallin. J. Biol. Chem. 272:6220-6225. [PubMed]
312. Sun, T. X., and J. J. N. Liang. 1998. Intermolecular exchange and stabilization of recombinant human αA- and αB-crystallin. J. Biol. Chem. 273:286-290. [PubMed]
313. Suzuki, C. K., M. Rep, J. M. Vandijl, K. Suda, L. A. Grivell, and G. Schatz. 1997. ATP dependent proteases that also chaperone protein biogenesis. Trends Biochem. Sci. 22:118-123. [PubMed]
314. Suzuki, T. C., D. C. Krawitz, and E. Vierling. 1998. The chloroplast small heat-shock protein oligomer is not phosphorylated and does not dissociate during heat stress in vivo. Plant Physiol. 116:1151-1161. [PubMed]
315. Takami, H., K. Nakasone, Y. Takaki, G. Maeno, R. Sasaki, et al. 2000. Complete genome sequence of the alkaliphilic bacterium Bacillus halodurans and genomic sequence comparison with Bacillus subtilis. Nucleic Acids Res. 28:4317-4331. [PMC free article] [PubMed]
316. Teter, S. A., W. A. Houry, D. Ang, T. Tradler, D. Rockabrand, G. Fischer, P. Blum, C. Georgopoulos, and F. U. Hartl. 1999. Polypeptide flux through bacterial Hsp70: DnaK cooperates with trigger factor in chaperoning nascent chains. Cell 97:755-765. [PubMed]
317. Tettelin, H., N. J. Saunders, J. Heidelberg, A. C. Jeffries, K. E. Nelson, et al. 2000. Complete genome sequence of Neisseria meningitidis serogroup B strain MC58. Science 287:1809-1815. [PubMed]
318. Thomas, J. G., and F. Baneyx. 2000. ClpB and HtpG facilitate de novo protein folding in stressed Escherichia coli cells. Mol. Microbiol. 36:1360-1370. [PubMed]
319. Thomas, J. G., and F. Baneyx. 1998. Roles of the Escherichia coli small heat shock proteins IbpA and IbpB in thermal stress management: comparison with ClpA, ClpB, and HtpG in vivo. J. Bacteriol. 180:5165-5172. [PMC free article] [PubMed]
320. Thompson, D. K., and C. J. Daniels. 1998. Heat shock inducibility of an archaeal TATA-like promoter is controlled by adjacent sequence elements. Mol. Microbiol. 27:541-551. [PubMed]
321. Thompson, D. K., J. R. Palmer, and C. J. Daniels. 1999. Expression and heat-responsive regulation of a TFIIB homologue from the archaeon Haloferax volcanii. Mol. Microbiol. 33:1081-1092. [PubMed]
322. Thompson, J. D., D. G. Higgins, and T. J. Gibson. 1994. CLUSTAL W: improving the sensitivity of progressive multiple sequence alignment through sequence weighting, positions-specific gap penalties and weight matrix choice. Nucleic Acids Res. 22:4673-4680. [PMC free article] [PubMed]
323. Tobias, J. W., T. E. Shrader, G. Rocap, and A. Varshavsky. 1991. The N-end rule in bacteria. Science 254:1374-1377. [PubMed]
324. Tomb, J. F., O. White, A. R. Kerlavage, R. A. Clayton, G. G. Sutton, et al. 1997. The complete genome sequence of the gastric pathogen Helicobacter pylori. Nature 388:539-547. [PubMed]
325. Török, Z., P. Goloubinoff, I. Horváth, N. M. Tsvetkova, A. Glatz, G. Balogh, V. Varvasovszki, D. A. Los, E. Vierling, J. H. Crowe, and L. Vigh. 2001. Synechocystis HSP17 is an amphitropic protein that stabilizes heat-stressed membranes and binds denatured proteins for subsequent chaperone-mediated refolding. Proc. Natl. Acad. Sci. USA 98:3098-3103. [PubMed]
326. Török, Z., I. Horváth, P. Goloubinoff, E. Kovács, A. Glatz, G. Balogh, and L. Vigh. 1997. Evidence for a lipochaperonin: Association of active protein folding GroESL oligomers with lipids can stabilize membranes under heat shock conditions. Proc. Natl. Acad. Sci. USA 94:2192-2197. [PubMed]
327. Trent, J. D., M. Gabrielsen, B. Jensen, J. Neuhard, and J. Olsen. 1994. Acquired thermotolerance and heat shock proteins in thermophiles from the three phylogenetic domains. J. Bacteriol. 176:6148-6152. [PMC free article] [PubMed]
328. Reference deleted.
329. Tu, G. F., G. E. Reid, J. G. Zhang, R. L. Moritz, and R. J. Simpson. 1995. C-terminal extension of truncated recombinant proteins in Escherichia coli with a 10Sa RNA decapeptide. J. Biol. Chem. 270:9322-9326. [PubMed]
330. van Bogelen, R. A., K. Z. Abshire, A. Pertsemlidis, R. L. Clark, and F. C. Neidhardt. 1996. Gene-protein database of Escherichia coli K-12, edition 6, p. 2067-2117.In F. C. Neidhardt et al. (ed.), Escherichia coli and Salmonella: cellular and molecular biology, 2nd ed. American Society for Microbiology, Washington, D.C.
331. van de Klundert, F. A., R. H. Smulders, M. L. Gijsen, R. A. Lindner, R. Jaenicke, J. A. Carver, and W. W. de Jong. 1998. The mammalian small heat-shock protein Hsp20 forms dimers and is a poor chaperone. Eur. J. Biochem. 258:1014-1021. [PubMed]
332. van den Ijssel, P. R., P. Overkamp, U. Knauf, M. Gaestel, and W. W. de Jong. 1994. αA-crystallin confers cellular thermoresistance. FEBS Lett. 355:54-56. [PubMed]
333. van den Oetelaar, P. J., P. F. van Someren, J. A. Thomson, R. J. Siezen, and H. J. Hoenders. 1990. A dynamic quaternary structure of bovine α-crystallin as indicated from intermolecular exchange of subunits. Biochemistry 10:3488-3493. [PubMed]
334. van Ham, R. C., A. Moya, and A. Latorre. 1997. Putative evolutionary origin of plasmids carrying the genes involved in leucine biosynthesis in Buchnera aphidicola (endosymbiont of aphids). J. Bacteriol. 179:4768-4777. [PMC free article] [PubMed]
335. Vanhoudt, J., S. Abgar, T. Aerts, and J. Clauwaert. 2000. Native quaternary structure of bovine α-crystallin. Biochemistry 39:4483-4492. [PubMed]
336. Vanhoudt, J., S. Abgar, T. Aerts, and J. Clauwaert. 2000. A small-angle X-ray solution scattering study of bovine α-crystallin. Eur. J. Biochem. 267:3848-3858. [PubMed]
337. van Melderen, L., and S. Gottesman. 1999. Substrate sequestration by a proteolytically inactive Lon mutant. Proc. Natl. Acad. Sci. USA 96:6064-6071. [PubMed]
338. van Melderen, L., M. H. D. Thi, P. Lecchi, S. Gottesman, M. Couturier, and M. R. Maurizi. 1996. ATP-dependent degradation of CcdA by Lon protease: effects of secondary structure and heterologous subunit interactions. J. Biol. Chem. 271:27730-27738. [PubMed]
338a. van Montfort, R. L. M., E. Basha, K. L. Friedrich, C. Slingsby, and E. Vierling. 2001. Crystal structure and assembly of a eukaryotic small heat shock protein. Nat. Struct. Biol. 8:1025-1030. [PubMed]
339. Varshavsky, A. 1997. The N-end rule pathway of protein degradation. Genes Cells 2:13-28. [PubMed]
340. Varshavsky, A. 1997. The ubiquitin system. Trends Biochem. Sci. 22:383-387. [PubMed]
341. Veinger, L., S. Diamant, J. Buchner, and P. Goloubinoff. 1998. The small heat-shock protein IbpB from Escherichia coli stabilizes stress-denatured proteins for subsequent refolding by a multichaperone network. J. Biol. Chem. 273:11032-11037. [PubMed]
342. Verbon, A., R. A. Hartskeerl, A. Schuitema, A. H. J. Kolk, D. B. Young, and R. Lathriga. 1992. The 14,000-molecular-weight antigen of Mycobacterium tuberculosis is related to the α-crystallin family of low-molecular-weight heat shock proteins. J. Bacteriol. 174:1352-1359. [PMC free article] [PubMed]
343. Vigh, L., D. A. Los, I. Horvath, and N. Murata. 1993. The primary signal in the biological perception of temperature: Pd-catalyzed hydrogenation of membrane lipids stimulated the expression of the desA gene in Synechocystis PCC6803. Proc. Natl. Acad. Sci. USA 90:9090-9094. [PubMed]
344. Vigh, L., B. Maresca, and J. L. Harwood. 1998. Does the membrane's physical state control the expression of heat shock and other genes? Trends Biochem. Sci. 23:369-374. [PubMed]
344a. Vijayalakshmi, J., M. K. Mukhergee, J. Graumann, U. Jakob, and M. A. Saper. 2001. The 2.2 A crystal structure of Hsp33: a heat shock protein with redox-regulated chaperone activity. Structure 9:367-375. [PubMed]
345. Wallington, E. J., and P. A. Lund. 1994. Rhizobium leguminosarum contains multiple chaperone (cpn60) genes. Microbiology 140:113-122. [PubMed]
346. Wang, K., and A. Spector. 2000. α-Crystallin prevents irreversible protein denaturation and acts cooperatively with other heat-shock proteins to renature the stabilized partially denatured protein in an ATP-dependent manner. Eur. J. Biochem. 267:4705-4712. [PubMed]
347. Watanabe, Y. H., H. Motohashi, H. Taguchi, and M. Yoshida. 2000. Heat-inactivated proteins managed by the DnaKJ-GrpE-ClpB chaperones are released as a chaperonin-recognizable non-native form. J. Biol. Chem. 275:12388-12392. [PubMed]
348. Waters, E. R. 1995. The molecular evolution of the small heat-shock proteins in plants. Genetics 141:785-795. [PubMed]
349. Waters, E. R., G. J. Lee, and E. Vierling. 1996. Evolution, structure and function of the small heat shock proteins in plants. J. Exp. Bot. 47:325-338.
350. Waters, E. R., and E. Vierling. 1999. Chloroplast small heat shock proteins: evidence for atypical evolution of an organelle-localized protein. Proc. Natl. Acad. Sci. USA 96:14394-14399. [PubMed]
351. Wawrzynow, A., B. Banecki, and M. Zylicz. 1996. The Clp ATPases define a novel class of molecular chaperones. Mol. Microbiol. 21:895-899. [PubMed]
352. Wawrzynow, A., D. Wojtkowiak, J. Marszalek, B. Banecki, M. Jonsen, B. Graves, C. Georgopoulos, and M. Zylicz. 1995. The ClpX heat-shock protein of Escherichia coli, the ATP-dependent substrate specificity component of the ClpP-ClpX protease, is a novel molecular chaperone. EMBO J. 14:1876-1877. [PubMed]
353. Weber-Ban, E. U., B. G. Reid, A. D. Miranker, and A. L. Horwich. 1999. Global unfolding of a substrate protein by the Hsp100 chaperone ClpA. Nature 401:90-93. [PubMed]
354. Wehmeyer, N., and E. Vierling. 2000. The expression of small heat shock proteins in seeds responds to discrete developmental signals and suggests a general protective role in desiccation tolerance. Plant Physiol. 122:1099-1108. [PubMed]
355. White, O., J. A. Eisen, J. F. Heidelberg, E. K. Hickey, J. D. Peterson, et al. 1999. Genome sequence of the radioresistant bacterium Deinococcus radiodurans R1. Science 286:1571-1577. [PubMed]
356. Wickner, S., S. Gottesman, D. Skowyra, J. Hoskins, K. McKenney, and M. R. Maurizi. 1994. A molecular chaperone, ClpA, functions like DnaK and DnaJ. Proc. Natl. Acad. Sci. USA 91:12218-12222. [PubMed]
357. Wickner, S., M. R. Maurizi, and S. Gottesman. 1999. Posttranslational quality control: folding, refolding, and degradating proteins. Science 286:1888-1893. [PubMed]
358. Wösten, M. M. S. M. 1998. Eubacterial sigma-factors. FEMS Microbiol. Rev. 22:127-150. [PubMed]
359. Wotton, D., K. Freeman, and D. Shore. 1996. Multimerization of Hsp42p, a novel heat shock protein of Saccharomyces cerevisiae, is dependent on a conserved carboxyl-terminal sequence. J. Biol. Chem. 271:2717-2723. [PubMed]
360. Xu, Z., A. L. Horwich, and P. B. Sigler. 1997. The crystal structure of the asymmetric GroEL-GroES-(ADP)7 chaperonin complex. Nature 388:741-750. [PubMed]
361. Yamanaka, K., L. Fang, and M. Inouye. 1998. The CspA family in Escherichia coli: multiple gene duplication for stress adaptation. Mol. Microbiol. 27:247-255. [PubMed]
362. Yeh, C. H., P. F. L. Chang, K. W. Yeh, W. C. Lin, Y. M. Chen, and C. Y. Lin. 1997. Expression of a gene encoding a 16.9-kDa heat-shock protein, Oshsp16.9, in Escherichia coli enhances thermotolerance. Proc. Natl. Acad. Sci. USA 94:10967-10972. [PubMed]
363. Young, D., R. Lathriga, R. Hendrix, D. Sweetser, and R. A. Young. 1988. Stress proteins are immune targets in leprosy and tuberculosis. Proc. Natl. Acad. Sci. USA 85:4267-4270. [PubMed]
364. Yuan, Y., D. D. Crane, and C. E. Barry. 1996. Stationary phase-associated protein expression in Mycobacterium tuberculosis: function of the mycobacterial α-crystallin homolog. J. Bacteriol. 178:4484-4492. [PMC free article] [PubMed]
365. Yuan, Y., D. D. Crane, R. M. Simpson, Y. Q. Zhu, M. J. Hickey, D. R. Sherman, and C. E. Barry. 1998. The 16-kDa α-crystallin (Acr) protein of Mycobacterium tuberculosis is required for growth in macrophages Proc. Natl. Acad. Sci. USA 95:9578-9583. [PubMed]
366. Yura, T., M. Kanemori, and M. T. Morita. 2000. The heat shock response: regulation and function, p. 3-18. In G. Storz and R. Hengge-Aronis (ed.), Bacterial stress responses. ASM Press, Washington, D.C.
367. Zantema, A., M. Verlaan-De Vries, D. Maasdam, S. Bol, and A. van der Eb. 1992. Heat shock protein 27 and αB-crystallin can form a complex, which dissociates by heat shock J. Biol. Chem. 267:12936-12941. [PubMed]
368. Zhu, X., X. Zhao, W. F. Burkholder, A. Gragerov, C. M. Ogata, M. E. Gottesman, and W. A. Hendrickson. 1996. Structural analysis of substrate binding by the molecular chaperone DnaK. Science 272:1606-1614. [PubMed]
369. Zolkiewski, M., M. Kessel, A. Ginsburg, and M. R. Maurizi. 1999. Nucleotide-dependent oligomerization of ClpB from Escherichia coli. Protein Sci. 8:1899-1903. [PubMed]
Articles from Microbiology and Molecular Biology Reviews : MMBR are provided here courtesy of
American Society for Microbiology (ASM)