|Home | About | Journals | Submit | Contact Us | Français|
Fusion of tubular membranes is required to form three-way junctions found in reticular subdomains of the endoplasmic reticulum. The large GTPase Atlastin has recently been shown to drive endoplasmic reticulum membrane fusion and three-way junction formation. The mechanism of Atlastin-mediated membrane fusion is distinct from SNARE-mediated membrane fusion, and many details remain unclear. In particular, the role of the amphipathic C-terminal tail of Atlastin is still unknown. We found that a peptide corresponding to the Atlastin C-terminal tail binds to membranes as a parallel α helix, induces bilayer thinning, and increases acyl chain disorder. The function of the C-terminal tail is conserved in human Atlastin. Mutations in the C-terminal tail decrease fusion activity in vitro, but not GTPase activity, and impair Atlastin function in vivo. In the context of unstable lipid bilayers, the requirement for the C-terminal tail is abrogated. These data suggest that the C-terminal tail of Atlastin locally destabilizes bilayers to facilitate membrane fusion.
The structure and function of intracellular organelles, particularly those in the secretory pathway, rely heavily on membrane and content exchange. In most cases, this exchange is accomplished by regulated membrane fusion. Cargo transport throughout the secretory pathway depends on specific targeting and fusion of the vesicular intermediates by SNARE proteins and their associated regulatory factors. The mechanism by which SNARE proteins drive membrane fusion is fairly well established (1, 2). However, membrane fusion events within the endomembrane system are still poorly characterized (3).
The morphology and function of the endoplasmic reticulum is inextricably linked to architectural shape changes. The interconnected network of ER5 tubules and sheets makes physical contact with virtually every cytoplasmic organelle (3). The dynamic nature of ER tubules allows for rapid shape changes that likely correspond to differences in functional interaction (4, 5). One of the major players involved in ER shape is the membrane fusion protein Atlastin (6). We and others have shown that the GTPase Atlastin drives the fusion of ER tubules and that this fusion reaction is vitally important for the overall function of this organelle (6, 7) Atlastin interacts with a variety of other proteins resident within the ER, like the ER shape-forming proteins reticulon, receptor expression-enhancing protein (REEP), and DP1 (7); spastin (8, 9); and luna park (10).
The mechanism by which Atlastin fuses ER membranes is beginning to be elucidated. We know that membrane fusion requires GTPase activity (6, 7), oligomerization (11), and structural elements within the extreme carboxyl terminus of the protein (11, 12). In this work, we examine the requirements and characteristics of the C-terminal juxtamembrane amphipathic α helix. We found that a peptide corresponding to 23 amino acids immediately after the second transmembrane domain forms a helix in the presence of membranes and directly interacts with membrane surfaces. We also show that membrane interaction alters the physical properties of the bilayer, such as membrane thinning and disorganization of fatty acid acyl chains. Targeted point mutations within the hydrophobic face of the amphipathic helix resulted in reduced membrane fusion in vitro, consistent with a role for amphipathic destabilization during the membrane fusion cycle. Additionally we found that Drosophila Atlastin functions in mammalian cells, where it also requires its C-terminal tail. Somewhat surprisingly, we found that mutations within the C-terminal helix were much more tolerated in vivo than in vitro. This result is likely because of alterations in the lipid composition of native membranes versus synthetic membranes used in in vitro fusion. We tested this directly by altering the lipid composition of synthetic proteoliposomes and found that phosphatidylethanolamine, which promotes non-bilayer-forming structures, can help alleviate the requirement for the C-terminal tail. In total, these results establish that the Atlastin C-terminal tail is a membrane-perturbing α helix that participates in membrane fusion by destabilizing the bilayer structure and promoting the mechanics of lipid mixing.
A bacterial expression vector containing GST fused to Drosophila Atlastin (dAtl) with a C-terminal octahistidine tag (pJM681) has been described previously (6). The construct pJM706 (GST-dAtl1–471-His8) has been described previously (11). The construction of other clones was carried out as detailed below.
The point mutation L482K was generated by overlap PCR using the primers DAtl L482K forward (CGACTTTGGCGGCAAGAAGGATGACTTTGCAAC) and dAtl L482K reverse (GTTGCAAAGTCATCCTTCTTGCCGCCAAAGTCG). The point mutation PCR product was further amplified by PCR using the primers BamHI-Dm_Atl (CCGGATCCATGGGCGGATCGGC) and Dm_Atl-XhoI (without stop) (ATCTCGAGTGACCGCTTCACC). The PCR product was then digested with BamHI and XhoI and ligated into pJM681 cut with the same enzymes.
The point mutation F478K was generated by overlap PCR using the primers dAtl F478K forward (GGAGAGCTCAGCGACAAAGGCGGCAAGTTGGATG) and dAtl F478K reverse (CATCCAACTTGCCGCCTTTGTCGCTGAGCTCTCC). The point mutation PCR product was further amplified by PCR using the primers BamHI-Dm_Atl (CCGGATCCATGGGCGGATCGGC) and Dm_Atl-XhoI (without stop) (ATCTCGAGTGACCGCTTCACC). The PCR product was then digested with BamHI and XhoI and ligated into pJM681 cut with the same enzymes.
The point mutations F478K and L482K were generated by overlap PCR using the primers dAtl F478K L482K forward (CTCAGCGACAAAGGCGGCAAGAAGGATGACTT) and dAtl F478K L482K reverse (AAGTCATCCTTCTTGCCGCCTTTGTCGCTGAG). The point mutation PCR product was further amplified by PCR using the primers BamHI-Dm_Atl (CCGGATCCATGGGCGGATCGGC) and Dm_Atl-XhoI (without stop) (ATCTCGAGTGACCGCTTCACC). The PCR product was then digested with BamHI and XhoI and ligated into pJM681 cut with the same enzymes.
The Hs-Atl1 C-terminal tail was generated by PCR using the primers BspEI-Hsatl1-c-tail (ATTCCGGAGAATACCGAGAGCTGG) and Hs_Atl_XhoI (TTCTCGAGCATTTTTTTCTTTTC). The PCR product was digested with BspEI and XhoI and ligated into pJM681 cut with the same enzymes.
The Hs-Atl3 C-terminal tail was generated by PCR using the primers BspEI-Hsatl3-c-tail (ATTCCGGACAATATCGTGAGCTGGGC) and Hs_Atl_XhoI (TTCTCGAGCATTTTTTTCTTTTC). The PCR product was digested with BspEI and XhoI and ligated into pJM681 cut with the same enzymes.
A gene fragment corresponding to residues 461–541 of dAtl, containing the L482K, A486D, L489D, and F493D point mutations, was synthesized by Integrated DNA Technology, cut with SacI and XhoI, and ligated into pJM681 cut with the same enzymes.
A gene fragment corresponding to residues 461–541 of dAtl, containing the G480K point mutation, was synthesized by Integrated DNA Technology, cut with SacI and XhoI, and ligated into pJM681 cut with the same enzymes.
Venus was PCR-amplified from Venus-GRX2 in pET28a (a gift from Joff Silberg (13)) using the oligos KpnI Venus A (CGGGTACCATGGTGAGCAAG) and Venus-BamHI 3′ (TAGGATCCGGGCCCAGCCTTGTA), cut with KpnI and BamHI, and ligated into pcDNA3.1 cut with the same enzymes. dAtl was PCR-amplified from pJM681 using the oligos BamHI-Dm_Atl (CCGGATCCATGGGCGGATCGGC) and Dm_Atl-XhoI (ATCTCGAGTCATGACCGCTTCACC), cut with BamHI and XhoI, and ligated into Venus in pcDNA3.1 cut with the same enzymes.
dAtl(1–471)-KKXX was PCR-amplified from pJM706 using the oligos BamHI-Dm_Atl (CCGGATCCATGGGCGGATCGGC) and Dm_atl(1–471)-GKVKRS-Stop-XhoI (CCCTCGAGTCATGACCGCTTCACCTTGCCATATCTAATGTAGGCCCAC), cut with BamHI and XhoI, and ligated into pJM850 cut with the same enzymes.
dAtl(L482K) was PCR-amplified from pJM882 using the oligos BamHI-Dm_Atl (CCGGATCCATGGGCGGATCGGC) and Dm_Atl-XhoI (ATCTCGAGTCATGACCGCTTCACC), cut with BamHI and XhoI, and ligated into pJM850 cut with the same enzymes.
dAtl(K51A) was PCR-amplified from pJM694 (GST-Dm-Atlastin (K51A) His8) using the oligos BamHI-Dm_Atl (CCGGATCCATGGGCGGATCGGC) and Dm_Atl-XhoI (ATCTCGAGTCATGACCGCTTCACC), cut with BamHI and XhoI, and ligated into pJM850 cut with the same enzymes.
The following mutants were generated using QuikChange site-directed mutagenesis PCR (Qiagen) and fully verified by sequencing.
The point mutation A486D was generated using the QuikChange primers dAtl A486D forward (GGCAAGTTGGATGACTTTGATACGCTATTGTGGGAG) and dAtl A486D reverse (CTC CCA AATAGCGTATCAAAGTCATCCAACTTGCC) with pJM850 as a template.
The triple point mutation was generated using the QuikChange primers dAtl_L482K_A486D_L489D forward (GGCAAGAAGGATGACTTTGATACGCTAGATTGGGAGAAATTCATGCGACCC) and dAtl_L482K_A486D_L489D reverse (GGGTCGCATGAATTTCTCCCAATCTAGCGTATCAAAGTCATCCTTCTTGCC) with pJM850 as a template.
The quadruple mutant was generated using the QuikChange primers dAtl_L482K_A486D_L489D_F493D forward (CGCTAGATTGGGAGAAAGACATGCGACCCATCTATCACGGCTGC) and DAtl_L482K_A486D_L489D_F493D reverse (GCAGCCGTGATAGATGGGTCGCATGTCTTTCTCCCAATCTAGCG) using Venus-dAtl (L482K;A486D;L489D) DNA as the template.
Two peptides, RYSGELSDFGGKLDDFATLLWEK (C23) and RYSGELSDKGGKKDDFATLLWEK (C23-KK), corresponding to the C-terminal tail of Drosophila Atlastin, were purchased from GenScript. The peptides contained an N-terminal acetylation and a C-terminal amidation.
1-palmitoyl-2-oleoyl-sn-glycero-3-phosphocholine (POPC) and 1,2-dioleoyl-sn-glycero-3-phospho-l-serine (DOPS) were purchased from Avanti Polar Lipids (Alabaster, AL). POPC and DOPS were mixed in a 85:15 molar ratio. Dried lipids were resuspended in Tris buffer solution (10 mm (pH 7)) to 1 mg/ml. This stock was fully mixed and exposed to more than five freeze-thaw cycles. A mini-extruder from Avanti Polar Lipids and Whatman Nuclepore Track-Etch 0.2-μm filters from GE Healthcare were used to produce liposomes. CD, oriented CD, and x-ray diffraction experiments were performed as described previously (14, 15).
Proteins purified in 0.1% Anapoe X-100 (Anatrace) were reconstituted into preformed 100-nm liposomes as described previously (6). Liposomes were made by extrusion. Lipid mixtures used were as follows: unlabeled (POPC) and labeled lipid mixtures (POPC:Rhodamine-DPPE:NBD-DPPE, 97:1.5:1.5 mole ratio), unlabeled lipid mixtures (POPC:DOPS, 85:15 molar ratio) and labeled lipid mixtures (POPC:DOPS:Rhodamine-DPPE:NBD-DPPE, 82:15:1.5:1.5 molar ratio), unlabeled lipid mixtures (POPC:DOPS:DOPE, 75:15:10 molar ratio) and labeled lipid mixtures (POPC:DOPS:DOPE:Rhodamine-DPPE:NBD-DPPE, 75:15:7:1.5:1.5 molar ratio), and unlabeled lipid mixtures (POPC:DOPS:DOPE, 65:15:20 molar ratio) and labeled lipid mixtures (POPC:DOPS:DOPE:Rhodamine-DPPE:NBD-DPPE, 65:15:17:1.5:1.5 molar ratio).
Lipid mixtures with trace amounts of 3H-1-palmitoyl 2-palmitoylphosphatidylethanolamine (DPPE) in chloroform were dried under a stream of nitrogen gas, followed by further drying in a vacuum for 30 min. The lipid films were resuspended in A100 + 10% glycerol, 2 mm 2-mercaptoethanol, and 1 mm EDTA to a final total lipid concentration of ~10 mm. Large unilamellar vesicles were formed by ten freeze-thaw cycles in liquid N2 and room temperature water. Uniform-sized large unilamellar vesicles were formed by extrusion through polycarbonate filters with 100-nm pore size (Avanti Polar Lipids).
GST-tagged proteins were purified starting by transforming Escherichia coli BL21(DE3) (Stratagene) cells with the respective expression plasmid. Overnight colonies were picked to start pre-precultures in 5 ml LB + ampicillin. The pre-precultures were used to start 50 ml precultures that were grown overnight at 25 °C. The cells from the 50-ml precultures were pelleted at 3000 rpm (~2000 × g) for 15 min using an Allegra tabletop centrifuge at room temperature. The cell pellet was used to seed 2- to 4-liter cultures with a starting density of about 0.1–0.2 OD600. The cultures were grown at 25 °C up to a desirable density (OD = 0.4 to 0.6), at which time the culture was moved to a 16 °C incubator. Ten minutes after growth at 16 °C, protein expression was induced with 0.2 mm isopropyl 1-thio-β-d-galactopyranoside, and the cultures were grown overnight (~16 h) at 16 °C. The cells were harvested, washed with A200 (25 mm HEPES (pH 7.4) and 200 mm KCl) and lysed in breaking buffer (A200 + 10% glycerol, 2 mm 2-mercaptoethanol (βME), 4% Triton X-100, and 1× complete protease inhibitor mixture (Roche)) by passage through an Emulsiflex C-3 high-pressure homogenizer (Avestin) twice at 15,000–20,000 p.s.i. Cell extracts were cleared by centrifugation at 125,000 × g (~186,000 × g) for 30 min using a Type 45-Ti rotor in an Optima LE-80K ultracentrifuge (Beckman) cooled to 4 °C. Cleared extracts were incubated with nickel Fast Flow beads for 30 min at 4 °C. The nickel bead-bound protein was washed with 10 ml of A400 (25 mm HEPES (pH 7.4) and 400 mm KCl) plus 10% glycerol, 2 mm βME, and 1% Triton X-100. The cells were then washed with 10 ml of A100 (25 mm HEPES (pH 7.4) and 100 mm KCl) plus 10% glycerol, 2 mm βME, and 1% Triton X-100 and then washed again with 10 ml of A100 plus 10% glycerol, 2 mm βME, 1% Triton X-100, and 0.1 m imidazole. The nickel-bound protein was then eluted with A100 plus 10% glycerol, 2 mm βME, 1% Triton X-100, and 0.5 m imidazole twice. The elutions were combined and incubated with 90 mg of swollen GSH-agarose beads (Sigma) for 1 h at 25 °C. The GSH bead-bound protein was washed with A100 plus 10% glycerol, 2 mm βME, 1% Triton X-100, and 1 mm EDTA. The protein was washed five more times with 10 ml of A100 plus 10% glycerol, 2 mm βME, 0.1% Anapoe X-100, and 1 mm EDTA. The protein was eluted from GSH-agarose with A100 plus 10% glycerol, 2 mm βME, 0.1% Anapoe X-100, 1 mm EDTA, and 10 mm GSH.
Proteins were analyzed by SDS-PAGE, and concentrations were determined by Amido Black protein assay (16). Frozen aliquots were stored at −80 °C.
Atlastin and Atlastin mutants were reconstituted into both labeled and unlabeled 100-nm liposomes by a detergent-assisted insertion method (17, 18) as follows. dAtl in 0.1% Anapoe X-100 was mixed with preformed liposomes at a 1:400 protein:lipid molar ratio and an effective detergent:lipid ratio of ~0.8. The effective detergent:lipid ratio (Reff) was determined by the equation Reff = Dtotal − Dwater / [lipid], where Dtotal is the total detergent concentration and Dwater is the monomeric detergent concentration (0.18 mm) in the presence of lipid. Protein and lipid were allowed to mix for 1 h at 4 °C. The detergent was removed by Bio-Beads SM-2 adsorbent (Bio-Rad) at 70 mg of Triton X-100/1 g of beads. Insoluble protein aggregates were pelleted by centrifugation of the samples in an Eppendorf microcentrifuge (10 min at 16,000 × g (max)). Final lipid and protein concentrations were determined by liquid scintillation counting and Amido Black protein assay (16), respectively. Protein:lipid ratios ranged from ~1:400–1:600, and protein concentrations ranged from ~1.5–2.5 μm. Reconstitution efficiencies were not dependent on protein or lipid composition.
Fusion assays were performed on the basis of a method described previously (6), with the following modifications. Labeled and unlabeled populations of Atlastin or mutant Atlastin proteoliposomes (0.15 mm lipid each) were mixed in the presence of 0.5 mm GTP or buffer only and brought to a total volume of 45 μl with A100 buffer in wells of 96-well FluoroNunc PolySorp plates (Nunc). The reactants in the plate were incubated at 37 °C in a fluorescent plate reader (Infinite M200, Tecan) for 5 min. To each well, 5 μl of 50 mm MgCl2 was added, and nitrobenzoxadiazole (NBD) fluorescence was measured (excitation 460 nm, emission 538 nm) at 1-min intervals for 60 min with a 1-s shaking after every reading. To determine the absolute NBD fluorescence, 10 μl of 2.5% (w/v) n-dodecylmaltoside was added at 60 min. Data were normalized to total fluorescence after detergent solubilization.
GTPase activity was measured as described previously (6) by measuring the release of inorganic phosphate from GTP, as suggested by the EnzChek phosphate assay kit (Molecular Probes). Recombinant Atlastin and Atlastin mutants were mixed in a 100-μl reaction volume with 1 unit/ml purine nucleoside phosphorylase, 200 μm 2-amino-6-mercapto-7-methylpurine riboside, and GTP in a transparent 96-well plate. The plates were warmed to 37 °C in a microplate reader (Infinite M200, Tecan), and 5 mm Mg2+ was added to start the reaction. In the presence of inorganic phosphate, purine nucleoside phosphorylase catalyzes the conversion of 2-amino-6-mercapto-7-methylpurine riboside to ribose 1-phosphate and 2-amino-6-mercapto-7-methylpurine, resulting in a spectrophotometric shift in absorbance from 330 to 360 nm. The absorbance increase at 360 nm was measured in real time approximately every 20 s over 20 min. Absorbance was normalized to phosphate standards, and initial rates were calculated.
The dAtl C-terminal tail peptide (45 μm) and liposomes (9.5 mm) were mixed in a Greiner half area plate (black). The total volume was adjusted to 50 μl with A100 buffer. Blank samples contained liposomes but no peptide. All samples were excited at 278 nm in a spectrofluorometer (Infinite M200, Tecan), and emission was measured between 300–500 nm.
HeLa cell culture, knockdown, and imaging were performed as described previously (19).
We have shown recently that the Atlastin C-terminal 23 amino acids are required for membrane fusion in vitro and in vivo (11). Bioinformatic analysis suggests that this segment of Atlastin is an amphipathic helix (Ref. 11 and Fig. 1A). We next wanted to probe this requirement more deeply by examining the interaction of a peptide corresponding to this region with membranes. First, we used a native tryptophan residue (amino acid 490 of Drosophila Atlastin) in the C-terminal peptide (C23) to examine the propensity of the peptide to associate with membranes. Liposomes containing pure phosphatidylcholine or a mixture of 85 mol% phosphatidylcholine and 15 mol% phosphatidylserine were incubated with or without peptide, and intrinsic tryptophan fluorescence was determined. Fig. 1B shows that the C-terminal peptide is membrane-active and binds to both membrane compositions, with a slight preference for membranes with no charge (Fig. 1B, green trace). These results are in agreement with a recent study that determined that a similar peptide from Drosophila Atlastin bound to membranes and could supply the required function in trans (20).
CD (Fig. 1D) suggests that C23 is largely unstructured in solution (blue circles), even in the presence of liposomes (red circles). However, the α-helical secondary structure parallel to the surface of the bilayer was observed by oriented CD (Fig. 1E) when the peptide was located between membranes of a multilayered structure.
We hypothesize that the primary function of the amphipathic C-terminal tail is to destabilize membrane structure during Atlastin-mediated membrane fusion. To test the effects of the C-terminal peptide on membrane structure, we employed x-ray diffraction to measure lipid organization in the presence of the peptide (21). Fig. 1, F and G, shows characteristic changes to membrane structures that are consistent with bilayer perturbation. The presence of the peptide results in an overall bilayer thinning, indicated by a reduced phosphate-to-phosphate distance with an increase in peptide concentration (Fig. 1, F and G) by about 10% (~38–34 Å). Additionally, the presence of the peptide resulted in a broadening of the trough of minimal x-ray intensity within the hydrophobic phase of the bilayer, indicative of acyl chain disorder (Fig. 1F). Overall, the Atlastin C-terminal tail peptide binds parallel to the surface of membranes as an α helix to induce bilayer thinning and acyl chain disorder, two properties important for the lipid rearrangements that occur during membrane fusion (1,–3, 22,–24).
We tested the functional conservation of the membrane-perturbing properties of this sequence by constructing chimeric Drosophila Atlastins that contain the entire C-terminal tail of human Atlastin-1 or human Atlastin-3 (Fig. 2). The loss of the tail eliminates fusion under most conditions (11, 20), but the presence of the human tails restores in vitro fusion to ~50% of the wild-type protein. This level of recovery is comparable with replacing the entire 60-amino acid tail with the juxtamembrane-conserved 23 amino acids (11). The ability of these Drosophila-human chimeras to support in vitro fusion confirms that the membrane-destabilizing characteristics of the amphipathic helix are also conserved across species.
The characteristic repeat structure of an amphipathic helix can be disrupted by replacing hydrophobic side chains that normally interact with the membrane with charged side chains. We generated several mutant Atlastins that alter the hydrophobic face, three of which are reported below. These include F478K, L482K, and the double mutant (F478K/L482K). These mutants were produced, reconstituted into proteoliposomes, and fused. Introduction of a single charge (F478K) close to the membrane interface reduced homotypic fusion by about 35% (Figs. 3, A and C, green trace and histogram, and and6),6), whereas a single charge one turn further down the helix face (L482K) decreased fusion by ~80% (Figs. 3, A and C, red trace and histogram, and and6).6). The double mutant (F478K/L482K), was marginally more effective than either single mutant (~85% reduction; Figs. 3, A and C, blue trace and histogram, and and6).6). A mutation in the C-terminal tail, but not in the hydrophobic face, G480K, did not reduce the fusion activity of Atlastin (Fig. 6).
Mutations in the hydrophobic face also impair the ability of the C-terminal tail to bind membranes. A peptide with the F478K and L482K mutations (C23-KK) shows reduced binding to liposomes (Fig. 1C). The C23-KK peptide, like the wild-type C23 peptide, is unstructured in solution (Fig. 1D). Unlike C23, C23-KK remains unstructured even when located between lipid bilayers. (Fig. 1E).
Given that we conduct fusion reactions with equal amounts of protein and lipid in both the labeled and unlabeled liposome populations, we can also determine the effects of mutations on heterotypic membrane fusion. In these reactions, the mutant Atlastin can be reconstituted in either the fluorescently labeled liposome population or the unlabeled bulk lipid liposome population. The location of the mutation relative to the fluorescent labeled lipid used to determine lipid mixing will influence the apparent effects on fusion. The schematic in Fig. 3E illustrates these effects. When we measured heterotypic fusion with the L482K charge mutant, we found an intermediate level of fusion (Fig. 3B, red traces with circles) compared with homotypic fusion (Fig. 3B, red trace, no symbols). The slight improvement in apparent fusion when the L482K mutation is located in the fluorescently labeled liposome population (Fig. 3B, red trace, filled red circles) can be explained by the population nature of the fusion reaction (Fig. 3E).
Next we tested the effects of mutations or deletions of the Atlastin tail in vivo. Previous studies have examined Drosophila expression in mammalian cells (6, 11, 25), primarily for the inability of mutant Atlastins to produce an overexpression phenotype. However, the functionality of Drosophila Atlastin in mammalian cells has not been demonstrated. HeLa cells primarily express human Atlastin-2 and Atlastin-3 with little or no Atlastin-1 (19). Knockdown of Atl-2 and Atl-3 by siRNA has proven to be a useful platform to examine Atlastin function by reintroduction of wild-type or mutant proteins (19). Loss of Atl-2 and Atl-3 in HeLa cells results in abnormal ER morphology, manifested as elongated ER tubes with reduced three-way junctions (Ref. 19 and Fig. 4A). When wild-type, full-length Drosophila Atlastin is reintroduced, normal ER morphology is restored (Fig. 4B). The rescued ER morphology is due to Drosophila Atlastin function because it is responsive to a dominant GTP binding mutation (K51A) that does not remedy the aberrant ER morphology (Fig. 4C). Drosophila Atlastin function in HeLa cells also requires the C-terminal amphipathic tail. An Atlastin mutant truncated at residue 471 that removes the C terminus but maintains an ER retention signal also fails to recover the ER morphology phenotype (Fig. 4D).
Next we determined the effect of C-terminal tail mutations of the amphipathic α helix in vivo. Surprisingly, single charge mutations in the C-terminal tail were largely without effect in vivo (Figs. 5, A and B, and and6).6). We expanded the mutant collection to include multiple mutations down the length of the hydrophobic face. Loss of function required four charge replacements before in vivo recovery was lost (Figs. 5D and and6).6). Fig. 6 compares the functional effects of point mutations within the hydrophobic face of the amphipathic helix both in vitro and in vivo.
Taken together, these data confirm that the C-terminal tail is required in vivo but that its functionality is much less susceptible to small changes in the physical characteristics of the amphipathic helix. One possible explanation is that even a low level of fusion activity is sufficient to restore the ER network in vivo. An alternative, more likely explanation is the substantial difference in lipid composition between the in vitro experiments and the in vivo result. To test the latter hypothesis directly, we re-examined in vitro fusion with an altered lipid composition. We suggest that the fundamental role of the C-terminal helical region is to provide membrane destabilization during the fusion mechanism. This role is supported by effects of the peptide containing this region on lipid bilayer structure. However, alterations in lipid composition can also influence the propensity of a bilayer to undergo the necessary lipid transitions during fusion. If the role of the C-terminal helix is to directly interact with the membrane to destabilize it, then perhaps an inherently more unstable lipid mixture will alleviate the need for this activity.
We produced proteoliposomes that contained increasing concentrations of the non-bilayer-forming lipid phosphatidylethanolamine (PE). The physical properties of PE and its relatively large amount of spontaneous negative curvature allow for membrane structural changes that are required during fusion (26). For this reason, membranes that contain PE are inherently more unstable and easier to fuse. Fig. 7 shows the outcome of in vitro membrane fusion reactions with mixtures of wild-type protein and the terminally truncated Atlastin that lacks the amphipathic tail. When wild-type Atlastin is present in both liposome populations, the inclusion of PE at 10 mol% (Fig. 7, green bar) or 20 mol% (Fig. 7, blue bar) is largely without effect. However, as we have shown previously (11), when both liposome populations contain the C terminally truncated Atlastin (1–471), fusion is largely abrogated in standard PC:PS liposomes (Fig. 7, black bar). Fusion is marginally improved with 10 mol% PE to roughly 9% of the wild type, whereas 20 mol% PE significantly improved in vitro fusion to roughly 31% of the wild type. In this reaction, neither fusion partner contains the C-terminal tail, yet fusion can occur at a reduced level. We also examined heterotypic fusion reactions that contained one C-terminal tail. The right half of Fig. 7A shows these results. A heterotypic interaction with one C-terminal tail in the PC:PS mixture was improved, and fusion approached wild-type levels when PE was included in the lipid mixture. As noted previously, the extent of fusion in the heterotypic reaction is dependent on the location of the mutant protein, in this case the C-terminal deletion, relative to the fluorescent lipid (Fig. 3E). Reconstitution efficiency is not affected by the addition of PE (Fig. 7B). The fusion activity of the L482K mutant was also improved by the addition of PE (Fig. 7C).
Membrane fusion requires phospholipids and other membrane components to undergo transitions that are energetically unfavorable and contrary to normal bilayer structure. Resident membrane proteins are responsible for encouraging these transitions and, ultimately, driving membrane merger. Membrane fusion driven by the GTPase Atlastin requires energy in the form of GTP hydrolysis as well as a conserved C-terminal amphipathic tail. Here we examine the role of this surface-active peptide during the process of membrane fusion. We found that a peptide corresponding to residues 470 and 492 of the Drosophila Atlastin interacts with membranes and does so in a manner consistent with bilayer perturbation (Fig. 1). A recent study (20) found that a similar peptide (residues 479–507) also binds to membranes and can serve its required role when added in trans as a soluble peptide in an in vitro fusion reaction.
The amphipathic nature of the C-terminal tail is conserved across species, and membrane-perturbing activity is also transplantable from human Atlastin-1 and Atlastin-3 to Drosophila Atlastin (Fig. 2). A continuous hydrophobic face is required for normal Atlastin function because replacement of conserved hydrophobic side chains with charged residues reduces the ability of Atlastin to drive fusion in vitro (Fig. 3). However, this requirement is less stringent in vivo (Fig. 5). We found that Drosophila Atlastin can functionally replace human Atlastin-2 and Atlastin-3 in HeLa cells and restore ER morphology. However, a GTP binding mutant, K51A, does not rescue (Fig. 4C), nor does a truncated Atlastin lacking the conserved amphipathic tail (Fig. 4D). The hydrophobic character of the amphipathic helix is also important in vivo, but much more significant perturbation is required to influence the ability of dAtl to rescue Atl-2/3 knockdown (Figs. 5 and and6).6). One likely reason for the decreased sensitivity to Atlastin tail mutation in vivo is the effect of membrane composition. Our in vitro studies utilized a very simple lipid composition, in most cases a single phospholipid. The endogenous lipid composition of the ER membrane (27) is much more complex and will influence membrane curvature and surface interactions, among others. To test this possibility more directly, we altered the lipid composition of our in vitro fusion reaction to include increasing concentrations of the non-bilayer-forming lipid PE. The net effect of PE inclusion is to destabilize the membrane by providing an increased ability to undergo curvature transition. With increasingly destabilized bilayers, we found a decreased requirement for the C-terminal tail (Fig. 7A). In essence, the destabilizing function of the C-terminal tail is unnecessary when the bilayer is composed of an inherently unstable mixture.
The mechanical nature of the amphipathic C-terminal tail is also supported by the results of heterotypic fusion experiments. The graded fusion response with one functional C-terminal tail with increasing PE (Fig. 7A, right) shows that bilayer perturbation is not required for both fusion partners. This is also true of the point mutation L482K in pure PC bilayers because a point mutant on either side of the fusion reaction yields an intermediate fusion response (Fig. 3B). These observations show that mutations with the C-terminal tail are biochemically recessive, which is fundamentally different from mutations within the GTPase domain, such as K51A or R48A, which are biochemically dominant (6, 11), consistent with the genetic dominance of homologous mutations in animals.
Membrane fusion driven by Atlastin appears to combine mechanistic features of both SNARE-mediated fusion and type I virus-mediated fusion. Sequences within the transmembrane domain(s) are important (20), as are regions that perturb the bilayer structure (Fig. 1), such as viral fusion peptides (28). The GTPase requirement that likely drives conformational changes (29,–31) necessary for fusion may be analogous to Rab proteins that influence the assembly of SNARE proteins (32). Future analysis of the Atlastin fusion mechanism will most likely reveal new features of this unique process.
5The abbreviations used are: