Rab guanosine triphosphatases (GTPases) are pivotal regulators of membrane identity and dynamics, but the in vivo pathways that control Rab signaling are poorly defined. Here, we show that the GTPase-activating protein Gyp7 inactivates the yeast vacuole Rab Ypt7 in vivo. To efficiently terminate Ypt7 signaling, Gyp7 requires downstream assistance from an inhibitory casein kinase I, Yck3. Yck3 mediates phosphorylation of at least two Ypt7 signaling targets: a tether, the Vps-C/homotypic fusion and vacuole protein sorting (HOPS) subunit Vps41, and a SNARE, Vam3. Phosphorylation of both substrates is opposed by Ypt7-guanosine triphosphate (GTP). We further demonstrate that Ypt7 binds not one but two Vps-C/HOPS subunits: Vps39, a putative Ypt7 nucleotide exchange factor, and Vps41. Gyp7-stimulated GTP hydrolysis on Ypt7 therefore appears to trigger both passive termination of Ypt7 signaling and active kinase-mediated inhibition of Ypt7's downstream targets. We propose that signal propagation through the Ypt7 pathway is controlled by integrated feedback and feed-forward loops. In this model, Yck3 enforces a requirement for the activated Rab in docking and fusion.
Ypt/Rab proteins are small GTP-binding proteins that localize to distinct membrane domains where they coordinate vesicle motility, cargo sorting, and SNARE-mediated fusion (Segev, 2001; Zerial and McBride, 2001; Pfeffer and Aivazian, 2004; Grosshans et al., 2006). Rabs function by cycling between inactive GDP-bound and active GTP-bound states (Milburn et al., 1990). Rabs are activated by guanine nucleotide exchange factors (GEFs) that eject GDP to promote GTP binding and are inactivated by GTPase-activating proteins (GAPs) that stimulate hydrolysis of the bound GTP (Moya et al., 1993; Strom et al., 1993; Pan et al., 2006; Bos et al., 2007). The Rab-GAP superfamily shares a Tre-2/Bub2/Cdc16 (TBC) domain sufficient for substrate specificity and catalytic activity (Albert et al., 1999; Pan et al., 2006; Bos et al., 2007). Nevertheless, only a few Rab GAPs are known to operate on specific Rabs in vivo (as opposed to in vitro), and almost nothing is known about what happens to targets downstream when Rabs are inactivated by their cognate GAPs.
Important insights into the role of Rabs in membrane fusion have been obtained from cell-free assays of Saccharomyces cerevisiae homotypic vacuole fusion (Wickner and Haas, 2000). The vacuole is the terminal endocytic compartment equivalent to the metazoan lysosome. Vacuole fusion in vitro entails four operationally defined subreactions: priming, tethering, docking, and fusion. Priming involves ATP hydrolysis by Sec18 to activate SNAREs for docking and fusion (Sollner et al., 1993; Mayer et al., 1996; Ungermann et al., 1998). Tethering is defined by formation of adhesive contacts between the participating membranes and is promoted by the vacuolar Rab GTPase Ypt7 (Haas et al., 1995; Wang et al., 2003). Docking entails a complex set of subreactions that occur between tethering and fusion. These subreactions require active Ypt7-GTP and its Vps-C/HOPS effector complex (Rieder and Emr, 1997; Wurmser et al., 2000; Wang et al., 2002, 2003; Collins et al., 2005). Docking culminates with formation of a trans-SNARE complex, an essential event that probably energizes membrane fusion (Hanson et al., 1997; Nichols et al., 1997; Weber et al., 1998; Jahn et al., 2003).
Assays of purified proteins reveal that the Rab GAP Gyp7 exhibits an in vitro preference for the vacuolar Rab Ypt7 (Wichmann et al., 1992; Vollmer et al., 1999). Purified Gyp7, its TBC domain, or the TBC domain of another GAP, Gyp1, inhibit in vitro homotypic vacuole fusion by arresting docking (Eitzen et al., 2000; Wang et al., 2003). However, it is unclear whether Gyp1, Gyp7, or other GAPs influence Ypt7 function in vivo (Zhang et al., 2005). We now show that Gyp7 targets Ypt7 in vivo but that Gyp7 cannot efficiently terminate Ypt7 signaling without downstream assistance from Yck3, the vacuolar casein kinase I. Moreover, we find that activated Ypt7 opposes Yck3-dependent phosphorylation of at least two Ypt7 signaling targets. We also show that one of these targets, the Vps-C/HOPS subunit Vps41, interacts directly with Ypt7 and that this interaction is essential for the stable association of the HOPS-tethering complex with Ypt7. Together with previous experiments, our results delineate a signaling pathway that renders the membrane fusion machinery highly responsive to the activation state of an upstream Rab GTPase.
Endogenous Gyp7 regulates vacuole fusion in vivo and in vitro
Extensive in vitro characterization of the eight S. cerevisiae Rab GAPs has revealed biochemical preferences for specific Rab substrates (Table S1), but the in vivo functions of these GAPs are largely undefined. Yeast cells are viable when GYP genes are deleted individually, and only a fraction of the knockout mutants exhibit detectable vesicle-trafficking defects, probably because of functional redundancy (Bos et al., 2007). As an alternative approach, we overproduced each of nine Gyp or Gyp-like proteins in cells. We then performed pulse-chase labeling with the styryl dye FM4-64 to examine vacuole morphology, a common indicator of endocytic trafficking defects (Fig. 1 a). Overproduction of Gyp1, Gyp5, or Gyl1 did not cause overt changes in vacuole morphology. Overproduction of Gyp2 and Gyp8 caused enlargement of the vacuole. In vitro, Gyp2 and Gyp8 stimulate GTP hydrolysis on Ypt6, which controls endosomal retrograde traffic, and on Sec4, which controls exocytosis of secretory vesicles. Thus, Gyp2 and Gyp8 may coordinate the inhibition of multiple Rabs within the cell to oppose secretion and retrograde endosomal traffic, shunting membrane to the vacuole. Gyp6, like Gyp2 and Gyp8, has an in vitro preference for Ypt6, but, unlike Gyp2 and Gyp8, it does not stimulate GTP hydrolysis on Sec4. Overproduction of Gyp6 caused accumulation of additional endosomal structures (Fig. 1 a), suggesting that Gyp6 more selectively opposes endosomal retrograde transport or endosome–vacuole fusion, as suggested by previous experiments (Ali et al., 2004). Overproduction of three Gyps, Gyp3/Msb3, Gyp4/Msb4, and Gyp7, caused vacuoles to fragment, consistent with reduced vacuole fusion. Gyp3 and Gyp4 are implicated in polarized exocytosis and appear to be functionally redundant, although they have divergent in vitro Rab specificities (Table S1; Gao et al., 2003). In vitro, both Gyp1 and Gyp7 inactivate Ypt7 and inhibit homotypic vacuole fusion (Eitzen et al., 2000). However, Gyp7 overexpression in vivo caused vacuoles to fragment, whereas Gyp1 overexpression did not (Fig. 1 a). Thus, the in vitro selectivity of a Rab GAP is often, but not always, a reliable indicator of its in vivo functions. Our data suggest that Gyp7, and possibly Gyp3 and Gyp4, are bona fide negative regulators of Ypt7.
In separate experiments, we uncovered a role for Gyp7 in vacuole fusion when hyperosmotic stress was applied to purified vacuoles in vitro (Brett and Merz, 2008). Upon exposure of wild-type cells to hypotonic conditions, vacuoles fuse within seconds (Bone et al., 1998; Wang et al., 1998, 2002), whereas upon exposure to hypertonic medium, vacuoles fragment within minutes (Bone et al., 1998; LaGrassa and Ungermann, 2005). We therefore assessed the in vivo consequences of GYP7 overexpression or deletion on vacuole morphology in cells grown under various osmotic conditions (Fig. 1 b). The gyp7Δ deletion allele decreased fragmentation slightly but significantly under standard conditions (Fig. 1 b), whereas overexpression of GYP7 from a high copy plasmid resulted in severely fragmented or multilobed vacuoles under all conditions, consistent with the idea that Gyp7 negatively regulates vacuole fusion in vivo (Fig. 1 b). Overexpression of GYP7 in gyp7Δ mutant cells also increased vacuole fragmentation compared with wild-type cells. This fragmentation required Gyp7 with an intact catalytic TBC domain. Overexpression of Gyp7 lacking the TBC domain or with a mutated catalytic arginyl residue within the TBC domain (R458K) was without effect (Fig. 1 a, bottom). These results support the hypothesis that Gyp7 opposes Ypt7 action in vivo.
To further evaluate the role of Gyp7, we assayed the in vitro homotypic fusion of vacuoles isolated from gyp7Δ mutant and GYP7 overexpressor cells (Fig. 1 c). In the standard assay of homotypic fusion, vacuoles are isolated from two yeast strains by equilibrium floatation: vacuoles from pep4Δ PHO8 cells contain inactive alkaline phosphatase, proPho8, whereas vacuoles from PEP4 pho8Δ cells lack proPho8 but contain a maturase needed for Pho8 activation. Membrane fusion between the two types of vacuoles results in lumenal content mixing and Pho8 activation, which is then quantified with a colorimetric assay to obtain an index of fusion (Wickner and Haas, 2000; Merz and Wickner, 2004a). Ypt7 inactivation occurs when vacuoles are exposed to hypertonic stress (Brett and Merz, 2008). Vacuoles isolated from gyp7Δ cells were reduced in sensitivity to hypertonic stress; conversely, vacuoles isolated from GYP7 overexpressors exhibited enhanced sensitivity to hypertonic stress (Fig. 1 c). Together, our results indicate that Gyp7 opposes Ypt7-dependent homotypic vacuole fusion both in vivo and in vitro.
Gyp7 inactivates Ypt7p in vivo
If Gyp7 modulates Ypt7 activity in vivo, we would expect that vacuoles isolated from gyp7Δ mutant or GYP7 overexpressor cells should bear different amounts of active Ypt7, and fusion of these vacuoles should exhibit modified sensitivity to Ypt7 inhibitors. To test these predictions, we performed dose-inhibition studies (Fig. 2 a) with recombinant GDI1 (rGdi1), a Rab chaperone that inhibits fusion by preferentially extracting inactive Rab–GDP complexes from membranes. As predicted, vacuoles isolated from gyp7Δ cells were less sensitive to rGdi1 than vacuoles from wild-type cells, whereas vacuoles isolated from GYP7 overexpressors were more sensitive to rGdi1 (Fig. 2 a). Similarly, vacuoles lacking Gyp7 were reduced in sensitivity to the recombinant catalytic domain of Rab-GAP Gyp1 (rGyp1TBC). In contrast, removal of endogenous Gyp7 did not alter dosage sensitivity to three inhibitors of fusion that do not target Ypt7: anti-Sec17 antibody, which blocks the early priming stage; anti-Vam3 antibody, which blocks SNARE function during docking; and MARCKS effector domain peptide, a late-stage inhibitor that chelates acidic lipid headgroups (Wang et al., 2003; Thorngren et al., 2004). To verify that rGyp1TBC inhibits fusion by inhibiting Ypt7 and not some other target (e.g., another Rab) on the vacuole, we used a GTP-“locked” Ypt7 mutant, Ypt7Q68L, which exhibits an 85% reduction in both intrinsic and GAP-stimulated GTP hydrolysis in vitro (Albert et al., 1999; Vollmer et al., 1999; Pan et al., 2006). In agreement with this result, in vitro fusion of vacuoles bearing Ypt7Q68L was 80% less sensitive to rGyp1TBC compared with vacuoles from wild-type cells (Fig. 2 b). Similarly, we found that the in vivo vacuole fragmentation caused by Gyp7 overproduction was suppressed by the YPT7Q68L allele (Fig. 2 c). Collectively, these results demonstrate that endogenous Gyp7 decreases the amount of functionally active Ypt7 on the vacuole.
To obtain a biochemical readout of the activation state of vacuolar Ypt7, we isolated vacuoles from gyp7Δ mutant cells or isogenic wild-type cells, incubated the vacuoles under fusion conditions, and briefly exposed them to rGdi1. Centrifugation was used to separate soluble from membrane pellet fractions (Fig. 3 a). Slightly more Ypt7 copurified with vacuoles from gyp7Δ cells compared with wild-type cells (Fig. 3 a, compare lane 1 with lane 3). Importantly, although rGdi1 extracted a majority of the Ypt7 on vacuoles isolated from wild-type cells, it extracted less than half of the Ypt7 on vacuoles from gyp7Δ cells (Fig. 3 a, compare lane 2 with lane 4; and Fig. 3 b, lane 1, 200-mM sorbitol condition). This result indicates that on vacuoles lacking Gyp7, an increased fraction of Ypt7 is in the active GTP-bound state. In addition, we examined the Ypt7 effector complex Vps-C/HOPS, which requires Ypt7 for its stable retention on the vacuole (Eitzen et al., 2000; Price et al., 2000; Seals et al., 2000). Like Ypt7, the HOPS subunit Vps41 was enriched on vacuoles isolated from gyp7Δ cells (Fig. 3 a), and a reduced fraction of Vps41 was released into the supernatant by rGdi1 treatment when Gyp7 was absent. Thus, the ratio of Ypt7:GTP to Ypt7:GDP is elevated on vacuoles obtained from gyp7Δ cells.
We next examined Ypt7 activity in wild-type and gyp7Δ cells under physical conditions that increase or decrease Ypt7-mediated tethering and docking (Fig. 3 b). We recently found that Ypt7 is stabilized on membranes when the osmotic strength of the assay buffer is reduced (Brett and Merz, 2008). A corresponding biochemical stabilization of Ypt7 was readily observed on vacuoles isolated from gyp7Δ versus GYP7 cells as the sorbitol concentration was varied (Fig. 3 b, compare lanes 1). Endogenous Gyp7 therefore modulates the sensitivity of Ypt7 extraction to changes in osmotic strength.
Three observations indicate that Ypt7 stabilization on vacuoles lacking Gyp7 results from decreased GTP hydrolysis, not from increased nucleotide exchange or an intrinsic resistance of Ypt7 to Gdi1-mediated extraction. First, GTP was not normally added to our cell-free reactions (Fig. 3, a and b, lanes 1); thus, stabilization of active Ypt7 does not require nucleotide exchange. Second, addition of rGyp1TBC resulted in almost complete extraction of Ypt7 under all conditions, indicating that unextracted Ypt7 is not intrinsically resistant to rGdi1 (Fig. 3 b, lanes 2). Third, and most importantly, preincubation of the vacuoles with GTPγS, a poorly hydrolyzable analogue of GTP, almost completely blocked Ypt7 extraction by rGdi1 (Fig. 3 b, lanes 3), indicating that Gdi1 is, as expected, preferentially extracting inactivated Ypt7. These findings were further supported by fusion experiments with rGdi1, rGyp1TBC, and GTPγS (Fig. S1). Collectively, the results presented in Figs. 1–3,23 establish Gyp7 as a major in vivo GAP of Ypt7.
Yck3p acts at the vacuole to oppose fusion
In addition to Gyp7, vacuole fusion is opposed by the casein kinase I Yck3 (LaGrassa and Ungermann, 2005). Yck3 localizes mainly to the vacuole, but it could oppose vacuole fusion either directly or indirectly (for example, by altering membrane recycling pathways). The latter possibility was a significant concern because Vps41, the only protein so far reported to be a target of Yck3, has been proposed to have roles in membrane budding as well as fusion (Rehling et al., 1999; Price et al., 2000). Yck3 requires ATP to function as a protein kinase, so we reasoned that removal of ATP should mimic the effects of Yck3 deletion. To test this idea, we exploited our finding that the recombinant SNARE rVam7 drives on pathway Rab- and SNARE-dependent fusion, bypassing the usual requirement for ATP and the Sec18 ATPase (Merz and Wickner, 2004b; Thorngren et al., 2004). Standard ATP-driven fusion reactions with vacuoles isolated from yck3Δ cells were highly resistant to rGdi1 when compared with reactions containing purified vacuoles from YCK3 cells (Fig. 4 a), as reported previously (LaGrassa and Ungermann, 2005). In rVam7-driven ATP bypass reactions, however, there was no difference in rGdi1 sensitivity between vacuoles from YCK3 and yck3Δ cells (Fig. 4 b). Comparable results were obtained using rGyp1TBC instead of rGdi1 (unpublished data). Together, these results show that under conditions in which vacuolar Yck3 cannot operate, vacuoles from YCK3 and yck3Δ strains have indistinguishable sensitivity to Rab inhibitors. With purified vacuoles, the effect of Yck3 manifests only under conditions in which the kinase can function, indicating that Yck3 must oppose Ypt7-stimulated fusion through immediate action on the vacuole, not through an indirect effect on membrane traffic.
YPT7 is epistatic to YCK3
The mechanisms by which Ypt7 promotes fusion are unclear. The 30-fold greater resistance of in vitro fusion to Ypt7 inhibitors when Yck3 is absent raised the possibility that the main function of Ypt7-GTP is to counteract an inhibitory effect of Yck3. This model predicts that if Yck3 is removed, Ypt7 should not be needed for fusion. Conversely, if other functions of Ypt7 (such as propagating a positive signal through the Vps-C/HOPS complex) are essential, both Ypt7 and its effectors should be needed for fusion in both the presence and absence of Yck3. To test these predictions, we constructed double mutant cells lacking Yck3 and Ypt7, Vps39, or Vps41. We then examined vacuole morphology using FM4-64 dye loading (Fig. 4 c). In the absence of Ypt7, the FM4-64–labeled vacuolar compartment was fragmented in every cell examined, whether Yck3 was present or absent. We found a similar epistasis relationship in growth assays (Fig. S2). Deletion of YCK3 also failed to suppress vacuole morphology defects in cells lacking either of two major Ypt7-binding partners, the Vps-C/HOPS subunits Vps39 (Wurmser et al., 2000) and Vps41 (see this paper). YPT7, VPS39, and VPS41 are therefore epistatic to YCK3. Because the Rab and its binding partners are needed for fusion in both the presence and absence of Yck3, Yck3 appears to function as a modulator of the Ypt7 signaling pathway.
To test Yck3 function under conditions in which Ypt7 function is compromised but not eliminated, we performed an in vivo version of the in vitro experiment shown in Fig. 4 a by overexpressing GYP7 in a yck3Δ mutant (Fig. 4 c). As shown in Fig. 1, GYP7 overexpression in a wild-type cell caused vacuolar fragmentation. In sharp contrast, fragmentation did not increase when GYP7 was overexpressed in yck3Δ mutant cells (Fig. 4 c). Thus, the in vivo and in vitro results are fully consistent and together reveal YCK3 as a classical modifier. YCK3 renders the YPT7 pathway far more sensitive to inhibition, but removal of YCK3 does not abrogate requirements for YPT7, VPS39, or VPS41.
Ypt7 opposes Yck3-mediated phosphorylation of Vps41 and Vam3
We next sought biochemical correlates of the functional and genetic interactions among Ypt7, Vps41, Gyp7, and Yck3. It was shown previously that Vps41, a subunit of the Ypt7 effector complex Vps-C/HOPS, is phosphorylated in a reaction that requires YCK3 (LaGrassa and Ungermann, 2005). This can be assayed by immunoblotting because phospho-Vps41 migrates slowly through SDS–polyacrylamide gels. Under standard in vitro vacuole fusion conditions, Vps41 phosphorylation was rapid and quantitative. Vps41 phosphorylation was inhibited, however, under conditions that activate or stabilize Ypt7, an effect readily observed when Gyp7 was absent (Fig. 5 a). Under standard reaction conditions (Fig. 5 a, 200 mM sorbitol, lane 1), most membrane-associated Vps41 was found in a slow-migrating band (Fig. 5 a, *). However, the faster-migrating, nonphosphorylated form (Fig. 5 a, o) became more abundant when Ypt7 was further stabilized, either by preincubating the vacuoles with GTPγS (Fig. 5 a, compare 200 mM sorbitol, lanes 1 and 3) or by lowering the buffer osmotic strength (Brett and Merz, 2008; Fig. 5 a, compare 200 mM with 100 mM sorbitol, lanes 1). The strongest inhibition of phosphorylation occurred when low osmolarity (Fig. 5 a, 100 mM sorbitol) and GTPγS were combined (Fig. 5 a, compare 100 mM sorbitol, lane 3 vs. 200 mM sorbitol, lane 1). Conversely, inactivation of Ypt7 with rGyp1TBC enhanced Vps41 phosphorylation and dissociation from the membrane (Fig. 5 a, lanes 2). Ypt7-GTP therefore opposes Yck3-dependent phosphorylation of Vps41.
The Qa-SNARE Vam3 is a core component of the vacuolar membrane fusion machinery and is essential for homotypic fusion. As with Vps41, we found that Vam3 is phosphorylated in a Yck3-dependent, Ypt7-inhibited reaction. ATP treatment resulted in slower Vam3 migration through SDS–polyacrylamide gels (Fig. 5 b, compare lane 9 with lane 10), and this observed change in Vam3 mobility is the result of phosphorylation. As previously reported for Vps41 (LaGrassa and Ungermann, 2005), slow-migrating Vam3 bands appeared only when ATP was supplied, and the slow-migrating bands for both Vps41 and Vam3 vanished upon exposure to alkaline phosphatase (Fig. 5 c). Slow-migrating, ATP-dependent phosphorylation products of both Vps41 and Vam3 appeared on vacuoles from YCK3 cells but were absent on vacuoles from yck3Δ mutant cells (Fig. 5 b, compare lanes 1–8 with lanes 9 and 10; and Fig. 5 d). Moreover, Vam3 phosphorylation, like Vps41 phosphorylation, was opposed by Ypt7-GTP (Fig. 5 d), as inhibition of Ypt7 with rGdi1 in the presence or absence of rGyp1TBC enhanced Vam3 phosphorylation at all sorbitol concentrations tested (Fig. 5 d, compare lanes 1 with lanes 2 and 3). Thus, at least two functional targets of Ypt7 (Vps41 and Vam3) are phosphorylated in Yck3-dependent reactions that occur on the vacuole, and phosphorylation of both targets is opposed by active Ypt7-GTP.
HOPS subunit Vps41 contains a Ypt7-binding site
The inhibition of Vps41 phosphorylation by activated Ypt7 (Fig. 5) raised the possibility that Ypt7 and Vps41 interact directly. The HOPS subunit Vps39 was reported to preferentially interact with unliganded Ypt7 and Ypt7-GDP (Wurmser et al., 2000), but in other experiments, the HOPS holocomplex was selectively captured on Ypt7-GTPγS affinity resins (Price et al., 2000; Seals et al., 2000). The divergent nucleotide specificities seen in these experiments suggested that the HOPS holocomplex might contain more than one Ypt7-binding site.
Fortuitously, a whole genome yeast two-hybrid screen for proteins that interact with the N-terminal region of Vps41 yielded only three strong hits from an ordered prey array of >5,000 yeast ORFs: Ypt7, Vam3, and Csm3 (Fig. S3 a). In retests against a miniarray of independently constructed and validated prey constructs, the Vps41–Vam3 interaction was not consistently reproduced, but Vps41 and Ypt7 interacted robustly in every experiment (Fig. 6). The Ypt7 prey interacted with bait constructs containing either full-length Vps41 or an N-terminal fragment of Vps41 (residues 99–500), but Ypt7 failed to interact with bait constructs containing the C-terminal half of Vps41 (residues 501–992). Moreover, Vps41 failed to interact with a series of Ypt7 point mutants. In sharp contrast, Vps39 or N-terminal Vps39 fragments interacted with a broad spectrum of Ypt7 mutants (Fig. 6) and interacted more robustly with some mutant alleles of Ypt7 than with the wild-type construct. The preferential recognition of different Ypt7 alleles by Vps39 and Vps41 provides strong evidence that the binding sites of these proteins recognize different features or states of Ypt7.
In previous studies (Price et al., 2000; Seals et al., 2000; Wurmser et al., 2000; LaGrassa and Ungermann, 2005), Vps39 and HOPS were shown to bind Ypt7 preferentially over Vps21 and Ypt1, but binding to the other eight yeast Rab proteins has not previously been evaluated. We found that neither Vps39 nor Vps41 interacted strongly with any yeast Rab other than Ypt7, indicating a high degree of binding selectivity. In an additional control performed to verify the specificity of the prey miniarray, Vac1, a known effector of the endosomal Rab Vps21, interacted with Vps21 and an activated Vps21 allele (Fig. S3 b) but not with Ypt7 or any other yeast Rab.
To further scrutinize Ypt7–Vps41 interactions, we performed affinity pull-down experiments using yeast cell lysates and resins decorated with GST-Rab fusion proteins. Consistent with our results from two-hybrid experiments (Fig. 6 a), Vps41 was retained on GST-Ypt7–GTPγS but not on seven other GST-Rab–GTPγS affinity matrices. The other component of HOPS known to bind Ypt7 directly, Vps39, exhibited a similar selectivity for Ypt7 over other Rabs in these experiments. Vps33, a component of both the Vps-C/HOPS and Vps-C/CORVET complexes, controls traffic to the prevacuolar endosome (Peplowska et al., 2007). Vps33 bound to Ypt7 preferentially, but it also bound other Rabs to a lesser extent, including the endosomal Rab Vps21 (Fig. 6 b). Together with our yeast two-hybrid results, these results demonstrate for the first time that Vps-C/HOPS interacts quite selectively with Ypt7 but not with any other S. cerevisiae Rab.
We next examined the relative contributions of Vps39 and Vps41 in the binding of HOPS to Ypt7 (Fig. 6 c). This experiment is possible because vps39Δ and vps41Δ mutant cells contain stable hybrid Vps-C complexes in which Vps39 or Vps41 are replaced by Vps3 or Vps8 (Peplowska et al., 2007). As reported previously, the HOPS holocomplex preferentially bound Ypt7 in the presence of GTPγS (Fig. 6 c; Price et al., 2000; Seals et al., 2000; Peplowska et al., 2007). In the absence of Vps39, however, HOPS binding to Ypt7 declined substantially, and the apparent nucleotide selectivity was lost (Fig. 6 c). In the absence of Vps41, HOPS binding to Ypt7 was undetectable, demonstrating that Vps41 is essential for stable Ypt7-HOPS binding. To test whether Ypt7 and Vps41 interact directly, pull-down experiments were performed using purified recombinant proteins. Consistent with the two hybrid assays (Fig. 6 a) and results obtained using lysates from vps39Δ cells (Fig. 6 c), full-length Vps41 bound to Ypt7 but not to Sec4. The Vps-C/HOPS complex therefore contains a minimum of two distinct and highly selective Ypt7-binding sites: one site resides in the presumed GEF, Vps39, and a second site resides in the N-terminal portion of Vps41.
A great deal is known about the enzymology of Rab regulation, but far less is known about how Rabs are regulated in the context of cellular physiology. The present experiments delineate a pathway that enforces the tight coupling of a membrane docking and fusion machinery to the activation state of its cognate Rab GTPase (Fig. 7). First, we show that the Rab7 paralogue Ypt7, which controls fusion at the lysosomal vacuole of budding yeast, is inactivated in vivo by a cognate GAP, Gyp7, confirming a relationship previously implied by in vitro assays with purified proteins (Vollmer et al., 1999; Eitzen et al., 2000; Pan et al., 2006). Second, we show that the casein kinase Yck3 acts directly at the vacuole as a downstream negative regulator of Ypt7 signaling. Third, we show that the Gyp7 GAP cannot efficiently terminate Ypt7 signaling in the absence of Yck3 in vivo. Fourth, we show that activated Ypt7-GTP acts to block Yck3-dependent phosphorylation of at least two of its own functional targets: the HOPS subunit Vps41 and the Vam3 SNARE. Finally, we demonstrate that Vps41 contains a Ypt7-binding site and is essential for stable HOPS binding to Ypt7.
In our working model (Fig. 7), the signaling state of Ypt7 is controlled by an activating GEF (probably Vps39; Wurmser et al., 2000) and an inhibitory GAP (Gyp7), whereas the coupling of downstream functions to Ypt7 activation is enforced by the Yck3 kinase, which inhibits Rab targets, increasing the amount of activated Rab required to generate a functional output (fusion). Moreover, the activated Ypt7 Rab itself opposes Yck3-mediated phosphorylation of Rab signaling targets. When the Rab is inactive, downstream functions are inhibited; when the Rab is active, it prevents inhibitory phosphorylation, and downstream functions are not inhibited. In the absence of the kinase, the Rab's downstream effectors are uninhibited, and even residual Rab signaling is sufficient to promote fusion.
Obviously, aspects of this working model are tentative. For example, the functional consequences of Yck3-dependent Vam3 phosphorylation are not yet characterized. However, Ungermann and colleagues have identified the site of Yck3-mediated phosphorylation within Vps41 and have confirmed that modification of this site inhibits Vps41 function (Ungermann, C., personal communication). At present, activated Ypt7-GTP is the only signal transducer known to regulate Yck3-dependent phosphorylation (Fig. 5). Ypt7-GTP could oppose Yck3-dependent phosphorylation by directly or indirectly inhibiting the intrinsic activity of Yck3 or by activating or localizing a phosphatase. Alternatively, Ypt7 could shield substrates from the Yck3 kinase through direct binding interactions, a possibility supported by our discovery that Vps41, a Yck3 target, also contains a Ypt7-binding site (Figs. 6 and 7).
Our data further suggest that a positive feedback loop controls activation of Ypt7 in a manner similar to that described for Rab5, its GEF Rabex-5, and its effector Rabaptin (Lippe et al., 2001). Vps39, the Ypt7 GEF (Wurmser et al., 2000), and Vps41 are physically associated as subunits of the Vps-C/HOPS tethering complex (Seals et al., 2000), and both subunits are necessary for specific binding of the HOPS holocomplex to Ypt7 in the presence of GTPγS (Fig. 6 c). Vps39-mediated activation of Ypt7 would generate additional binding sites for HOPS, thereby further stabilizing HOPS at the membrane and allowing Vps39 to engage in multiple cycles of Ypt7 activation (Fig. 7 b). Studies of Ypt7-regulated protein localization at vacuole-docking junctions provide additional support for the existence of a Vps39-mediated positive feedback loop (Wang et al., 2003). Because Vps41 is needed for stable HOPS binding to Ypt7, we predict that inactivation of Vps41 by Yck3 will terminate this positive feedback, reducing the efficacy of Vps39-mediated Ypt7 activation. Experimental tests of these predictions are underway in our laboratory.
There are several examples of phosphorylation regulating Rab signaling pathways. The Rab GAP AS160 (Sano et al., 2003) regulates insulin-stimulated exocytosis of glucose transporters. When phosphorylated by Akt, AS160 is inhibited, permitting activation of its target, Rab10 (Roach et al., 2007; Sano et al., 2007). Phosphorylation also regulates downstream targets of Rabs, including SNARE proteins, in both yeast and mammals. For example, casein kinase II phosphorylates the synaptic Qa-SNARE syntaxin 1A in vitro (Hirling and Scheller, 1996). Phosphorylation often inversely correlates with fusion. Yeast cells expressing a Golgi Qa-SNARE Sed5 phosphomimetic mutant have fragmented Golgi compartments, whereas cells expressing a phosphorylation-resistant Sed5 mutant have ordered Golgi (Gurunathan et al., 2002; Weinberger et al., 2005). Rab effectors are also phosphorylated (Lonart and Sudhof, 1998; Lonart et al., 2003). For example, phosphorylation of the Rab11 effector Rip11 controls its localization on apical recycling endosomes within epithelial cells (Prekeris et al., 2000). Finally, the Ypt31/32 Rab GTPases regulate phosphorylation of the yeast R-SNARE Snc1 (Chen et al., 2005). Thus, interactions between Rab signaling and phosphorylation are pervasive.
A general problem in biological signal transduction is the maintenance of fidelity in circuits that, because they rely on small populations of molecules, operate in a noisy analogue mode. In these systems, negative feedbacks are used to maintain homeostatic equilibria, whereas positive feedbacks can amplify small signals or generate switchlike behaviors. We propose that the Ypt7 signaling pathway incorporates both a positive feedback loop that reinforces Ypt7 activation and a positive feed-forward loop (which uses two negative elements in series) that enforces the requirement for Ypt7 activation (Fig. 7). We propose that this circuit topology increases the fidelity of Ypt7-mediated signaling by suppressing spurious downstream signaling when an upstream signal falls below a specific threshold. This in turn renders the overall pathway more responsive to signals that impinge on Ypt7 by increasing the pathway's signal to noise ratio. Given the commonality of other strategies in small GTPase signaling (Grosshans et al., 2006; Bos et al., 2007), it is likely that such an arrangement will not be unique to the vacuolar Rab.
Note added in proof.
We have identified conditions under which purified Vps41 binds selectively to Ypt7-GTPγS. To obtain homogenous Ypt7-GDP, GST-Ypt7 bound to ∼50 μl of glutathione-agarose beads is incubated with 5 μg His6-Gyp1TBC overnight at 4°C and for 30 min at 23°C. The Gyp1 is removed. GST-Ypt7-GTPγS is prepared from GST-Ypt7-GDP by incubating the bead suspension for 90 min at 23°C in nucleotide exchange buffer (50 mM Tris-Cl, pH 8.0, 100 mM NaCl, 4 mM EDTA, and 5 mM 2-mercaptoethanol) containing 1.4 mM GTPγS. GTPγS loading is stopped by the addition of excess pull-down buffer (50 mM Tris-Cl, pH 8.0, 100 mM NaCl, 5 mM MgCl2, and 5 mM 2-mercaptoethanol). The beads are washed twice in pull-down buffer, and Vps41 pull-down is performed as in Fig. 6 d.
Materials And Methods
Strains and plasmids
For fusion assays, we used complimentary strain pairs of BJ3505 (MATα pep4∷HIS3 prb1-1.6R his3-200 lys2-801 trp1-101 [gal3] ura3-52 gal2 can1) and DKY6281 (MATα leu2-3 leu2-112 ura3-52 his3-200 trp1-901 lys2-801) or BY4742 pep4Δ (MATα ura3Δ leu2Δ his3Δ lys2Δ pep4Δ∷neo [Invitrogen]) and BY4742 pho8Δ∷neo. BJ3505 GFP-VPS39, BJ3505 gyp7Δ∷URA3, DKY6281 gyp7Δ∷URA3 or BJ3505 YPT7Q68L∷neo, and DKY6281 YPT7Q68L∷neo were provided by W. Wickner (Dartmouth College, Hanover, NH), G. Eitzen (University of Alberta, Edmonton, Canada), and D. Gallwitz (Max Planck Institute of Biophysical Chemistry, Göttingen, Germany). Double mutant yck3Δ pep4Δ (AMY807), yck3Δ pho8Δ (AMY809), yck3Δ ypt7Δ (AMY913), yck3Δ vps41Δ (AMY996), or yck3Δ vps39Δ (AMY999) cells were constructed by mating BY4741 (MATα ura3Δ leu2Δ his3Δ met15Δ [Invitrogen]) with BY4742-derived haploid cells and sporulating; the genotypes of spores isolated by tetrad dissection were confirmed by mapping PCR. Gyp7-overproducing BY4742 wild-type, gyp7Δ, ypt7Δ, yck3Δ, yck3Δypt7Δ and BJ3505, DKY6281, or DKY6281 YPT7Q68L cells carried the plasmid pYADH1-GYP7-His6 (GYP7 with a C-terminal hexahistidine tag inserted behind the ADH1 promoter in the 2-μ yeast shuttle vector [39967; American Type Culture Collection] D. Gallwitz). The set of regulated GYP plasmids was constructed by gap repair–mediated homologous recombination between the vector pCM190 (containing a tetracycline-repressible promotor; Gari et al., 1997), and each of the eight GYP genes or GYL1 (a GYP-like gene) was amplified by PCR with primers containing terminal sequences homologous to pCM190. The resulting plasmids were rescued into Escherichia coli, amplified, sequenced, and transformed into S. cerevisiae BY4742. Transformants were selected in the presence of doxycycline and in the absence of uracil. Gyp overproduction was induced by removing doxycycline from the growth medium.
All biochemical reagents were purchased from Sigma-Aldrich or Invitrogen, except as indicated, and were of biotechnology grade or better. The endoglucanase fraction of Zymolyase (20T; Seikigaku) was purified by cation exchange chromatography before use in vacuole isolation. Calf intestinal phosphatase (CIP) was purchased from New England Biolabs, Inc. Purified proteins used include rGdi1 purified from bacterial cells using a calmodulin-binding peptide intein fusion system (provided by V. Starai, Dartmouth Medical School, Hanover, NH; and W. Wickner), rGyp1TBC, recombinant soluble Qc-SNARE Vam7, and recombinant protease inhibitor Pbi2. Rabbit polyclonal sera raised against Vps41, Vps33, Ypt7, and Vam3 (provided by W. Wickner) were affinity purified and, in some cases, were cross-adsorbed against cell lysates from corresponding yeast deletion strains to reduce cross-reactivity. The protein reagents used in fusion assays were prepared in 10 mM Pipes-KOH, pH 6.8, and 200 mM sorbitol (Pipes-sorbitol buffer, PS) or were exchanged into this buffer by dialysis or size exclusion chromatography.
Vacuoles were purified as described previously by Haas et al. (1995). 6 μg of isolated vacuoles was incubated for 90 min at 27°C in standard reaction buffer as follows: PS buffer supplemented with salts (0.5 mM MgCl2 and 125 mM KCl), 10 mM CoA, and Pbi2 with or without ATP-regenerating system (0.5 mM ATP, 0.1 mg/ml creatine kinase, and 40 mM creatine phosphate). Bypass fusion was initiated with 100 nM rVam7 in the presence of 1 mg/ml BSA. Osmotic gradients were imposed by reducing or adding sorbitol to the standard isotonic reaction buffer (200 mM sorbitol). As indicated, reactions also contained CIP, rGdi1, rGyp1TBC, or GTPγS. The total volume of each fusion reaction was 30 μl. Fusion reactions were conducted using DKY6128 (or BY4742 pho8Δ; alkaline phosphatase deficient) and BJ3505 (or BY4742 pep4Δ; protease deficient) vacuoles (3 μg each) with or without genomic deletion of GYP7 (gyp7Δ) or YCK3 (yck3Δ), with YPT7 or YPT7Q68L, or expression of pYADH1-GYP7-His6 (+GYP7). Homotypic vacuole fusion was measured using a biochemical complementation assay (Haas et al., 1995; Merz and Wickner, 2004a). Fusion (content mixing) was quantified by monitoring the alkaline phosphatase–catalyzed evolution of p-nitrophenolate at 400 nm. Signals were then subtracted from a background control reaction either lacking ATP or incubated on ice; the signal to background ratio under our standard conditions routinely exceeds 25:1. Results are reported relative to signals obtained under standard fusion conditions (200 mM sorbitol with ATP or rVam7). Under standard conditions, the mean extent of fusion was 4.11 ± 0.12 (n = 16) fusion units as previously defined (Haas et al., 1995; Merz and Wickner, 2004a). Vacuole membrane release or the phosphorylation state of Ypt7, Vam3, and HOPS components was determined using fusion reactions containing exclusively protease-deficient vacuoles (6 μg BJ3505 or BY4742 pep4Δ). After incubation at 27°C for 40 or 70 min, fusion reactions were immediately sedimented by centrifugation at 20,000 g for 5 min at 4°C. Pellet and supernatant fractions were separated by SDS-PAGE and analyzed by immunoblotting as indicated.
To assess vacuole morphology in vivo, yeast were incubated for 1 h at 30°C in synthetic complete (SC) medium containing 3 μM FM4-64, sedimented, and resuspended in SC. After a 30-min chase period, cells were sedimented again, resuspended in either water, SC, or SC supplemented with 0.4 M NaCl, incubated for 5 or 30 min at 30°C, and imaged. To quantify cellular vacuole morphology phenotypes, at least six micrographs containing fields of ∼30 cells (from three independent cultures) were acquired, and cellular vacuole morphology was visually classified as either round or multilobed using the scheme of LaGrassa and Ungermann (2005; Fig. 1 b). Cells were scored as “round” if vacuoles were present as a single large or small spherical structure, a single large spherical structure with small adjoining vesicles, or two large oblong abutting structures. Cells were scored as “multilobed” (or fragmented) if they contained three or more small spherical structures or a single tubular structure with one or more spherical structures. All micrographs were acquired using a microscope (IX71; Olympus) equipped with an electron-multiplying charge-coupled device (iXon; Andor), ultrabright green and blue light-emitting diodes (>350-mW output) driven by custom electronics, a PlanApoN 1.45 NA 60× objective lens, and iQ software (version 18.104.22.168; Andor). Micrographs were processed using ImageJ (version 1.36b; National Institutes of Health) and Photoshop CS (version 8.0; Adobe) software. The images shown were adjusted for brightness and contrast and sharpened with an unsharp masking filter.
Parent strains and plasmids were obtained from the University of Washington Yeast Resource Center. Two-hybrid plasmid constructs were constructed in haploid yeast strains by PCR-mediated homologous recombination cloning. ORF or domain sequences were amplified by PCR using primers containing terminal homology to the two-hybrid test vectors. Prey domains were cloned into gapped pOAD plasmid by cotransformation into the yeast strain PJ69-4 MATα. Bait domains were cloned into pOBD2 in strain PJ69-4 MATα. Clonal isolates were verified by PCR and DNA sequencing. Interaction tests were performed by mating bait and prey haploid strains. Liquid cultures of the bait and prey strains were grown in selective media, mixed in 96-well plates, and pinned to yeast extract–peptone–dextrose plates supplemented with adenine using a 48-spoke inoculating manifold. These mating plates were grown at 30°C overnight, and diploids were selected by replica plating onto medium lacking tryptophan and leucine and supplemented with adenine. Diploid colonies were grown at 30°C for 2 d, replica plated to medium lacking tryptophan, leucine, and histidine, and supplemented with adenine and 1.5 mM 3-amino-1,2,4-triazole. After 5 d at 30°C, the plates were scored for growth.
GST-Rab pull-down assays
GST or GST-Rab fusion proteins were expressed in E. coli BL21-pRIL cells transformed with the vector pGST-Parallel-1 or with the same vector containing in-frame NcoI–BamHI PCR products encoding full-length Rab genes. Fusion proteins were coupled to glutathione–Sepharose 4B resin (GE Healthcare) as described previously for Ypt7 (Price et al., 2000), except coupling was performed in the absence of EDTA and EGTA, and 5 mM MgCl2 was present throughout. Nucleotide loading of Rab proteins was performed by incubating Rab-bound resin in exchange buffer (50 mM Tris-HCl, pH 8.5, 100 mM NaCl, 0.01% 2-mercaptoethanol, 5 mM MgCl2, and 500 μM guanine nucleotide) for 30 min. 50 μl of packed, nucleotide-loaded GST-Rab resin was incubated with 500 μl of vacuole lysates, whole cell lysates, or recombinant Vps41 for 2 h. The resin was washed five times with 500 μl of lysis or solubilization buffer, and bound proteins and GST-Rabs were eluted by boiling reactions in 1× SDS buffer for 10 min. Equal loading of glutathione resins with Rab proteins was confirmed by SDS-PAGE. Whole cell lysates were similarly prepared as vacuoles, but after spheroplasting, cells were resuspended in lysis buffer (20 mM Hepes-KOH, pH 7.4, 50 mM potassium acetate, 200 mM sorbitol, 0.01% 2-mercaptoethanol, 5 mM MgCl2, 0.7 μg/ml leupeptin, 0.5 μg/ml pepstatin, and 1 mM PMSF) and lysed by Dounce homogenization on ice. The lysate was solubilized with 1% Triton X-100 and clarified by centrifugation (20,000 g for 15 min). 500 μg of lysate protein was then added to the resin. Vacuole lysates were prepared by sedimenting 300 μg of isolated vacuoles (20,000 g for 10 min), resuspending membrane pellets in 500 μl of solubilization buffer (25 mM Hepes-KOH, pH 7.4, 125 mM NaCl, 10% glycerol, 0.5% Triton X-100, 5 mM MgCl2, 0.01% 2-mercaptoethanol, and protease inhibitors), and clarifying soluble lysates by centrifugation (13,000 g for 10 min). Except as noted, all experiments were performed on ice or at 4°C.
Preparation of recombinant Vps41
His6-tagged Vps41 was expressed in Tn-5B1-4 (High-5) insect cells using the Bac-to-Bac system (Invitrogen). An in-frame BamH1–KpnI PCR product encoding full-length Vps41 was inserted into the shuttle vector pFB-HTB-N. The resulting plasmid was sequenced and transformed into DH10Bac E. coli, and bacmid DNA was purified from this strain. Bacmid DNA was transfected into Sf9 cells to prepare first, second, and third generation multiple nuclear polyhedrosis baculovirus stocks. Suspension-adapted High-5 cells were infected with virus, grown in suspension using SF-900 II serum-free media, supplemented with 100 U/ml penicillin, 10 μg/ml streptomycin, and 0.11 μg/ml l-glutamine for 72 h at 27°C, and harvested. Cell pellets were washed three times in PBS, resuspended in lysis buffer (50 mM Tris-HCl, pH 8.0, 350 mM NaCl, and 5 mM 2-mercaptoethanol), and lysed by sonication. Lysates were clarified by centrifugation (18,000 g for 20 min), incubated with pre-equilibrated nickel-nitrilotriacetic acid resin (GE Healthcare) for 1 h, and eluted using lysis buffer supplemented with 350 mM imidazole. The resulting eluate was size fractionated and exchanged into storage buffer (50 mM Tris-HCl, pH 8.0, 150 mM NaCl, 5 mM 2-mercaptoethanol, and 10% glycerol) on a Superdex 200 column (GE Healthcare). Aliquots of Vps41 were frozen in thin-walled PCR tubes by immersion in liquid nitrogen.
Where applicable, datasets were fit to sigmoidal dose–response functions using a nonlinear least-squares algorithm. Log IC50 values were extracted from the sigmoidal fits using Prism software (version 4.0c; GraphPad Software, Inc.). Data are reported as mean ± SEM. Mean comparisons were performed using Student's two-tailed t tests with corrections for multiple comparisons.
Online supplemental material
Table S1 shows a summary of in vitro Rab specificities of the nine yeast Rab-GAP proteins. Fig. S1 shows that addition of GTP or GTPγS to vacuole fusion reactions overcomes inhibition of Ypt7 by rGdi1 or rGyp1TBC. Fig. S2 shows that deletion of YCK3 is unable to suppress poor growth of ypt7Δ yeast at high temperatures. Fig. S3 shows a complete list of Vps41-interacting proteins obtained from our genome-wide yeast two-hybrid screen and control data validating the use of our two-hybrid miniarrays to evaluate Rab-binding selectivity.
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Abbreviations used in this paper: CIP, calf intestinal phosphatase; GAP, GTPase-activating protein; GEF, guanine nucleotide exchange factor; HOPS, homotypic fusion and vacuole protein sorting; rGdi1, recombinant GDI1; SC, synthetic complete; TBC, Tre-2/Bub2/Cdc16.
We thank D. Gallwitz, G. Eitzen, and members of our group for critical discussions; W. Wickner, G. Eitzen, D. Gallwitz, and M. Kleijnen for generous gifts of antibodies and strains; and C. Ungermann for sharing unpublished results.
This work was supported by grant GM077349 from the National Institutes of Health. High throughput screening was performed by the National Center for Research Resources Yeast Resource Center which was supported by grant P41 RR11823 from the National Institutes of Health.
C.L. Brett and A.J. Merz conceived and designed the experiments. C.L. Brett performed most of the experiments. B.T. Lobinger prepared and characterized recombinant Vps41. R.L. Plemel constructed and analyzed yeast strains and performed two-hybrid miniarray analyses. M. Vignali and S. Fields designed and performed high throughput screening. C.L. Brett and A.J. Merz wrote the paper.