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. 2020 Jul 3;8:539. doi: 10.3389/fcell.2020.00539

Lipid Rafts, Sphingolipids, and Ergosterol in Yeast Vacuole Fusion and Maturation

Logan R Hurst 1, Rutilio A Fratti 1,2,*
PMCID: PMC7349313  PMID: 32719794

Abstract

The Saccharomyces cerevisiae lysosome-like vacuole is a useful model for studying membrane fusion events and organelle maturation processes utilized by all eukaryotes. The vacuolar membrane is capable of forming micrometer and nanometer scale domains that can be visualized using microscopic techniques and segregate into regions with surprisingly distinct lipid and protein compositions. These lipid raft domains are liquid-ordered (Lo) like regions that are rich in sphingolipids, phospholipids with saturated acyl chains, and ergosterol. Recent studies have shown that these lipid rafts contain an enrichment of many different proteins that function in essential activities such as nutrient transport, organelle contact, membrane trafficking, and homotypic fusion, suggesting that they are biologically relevant regions within the vacuole membrane. Here, we discuss recent developments and the current understanding of sphingolipid and ergosterol function at the vacuole, the composition and function of lipid rafts at this organelle and how the distinct lipid and protein composition of these regions facilitates the biological processes outlined above.

Keywords: membrane fusion, sphingolipids, membrane trafficking, lipid rafts, vacuole

Introduction

The lysosomal vacuole of S. cerevisiae plays a number of important roles in cellular homeostasis. The importance of the eukaryotic lysosomal compartment is underscored by the fact that there are over 70 human diseases whose molecular basis is intricately tied to dysfunctions of lysosomal storage and homeostasis (Platt et al., 2018). The fungal vacuole is necessary for nutrient storage, protein turnover, and detoxification, but it also plays a large and often-underappreciated role in essential processes such as autophagy, ion homeostasis, and organelle contact and fusion (Li and Kane, 2009). Membrane fusion is a conserved biological process that occurs at most, if not all, cellular membranes, and is necessary for autophagy, secretion and endocytic recycling. The process of homotypic vacuolar fusion in yeast cells is essential for maintaining osmotic balance, pH balance, and vacuolar inheritance by the daughter cell, and this system has proven to be instrumental in understanding many of the basic mechanisms of membrane fusion (Wickner, 2010). Through years of exemplary work by a number of labs across the world many of the factors that are necessary for fusion have been identified, and in most cases a molecular mechanism for these effectors has been investigated in detail. These fusion effectors include proteins such as tethers, Rab/Rho GTPases, SNAREs, chaperones and actin, and the regulatory lipids phosphatidic acid (PA), diacylglycerol (DAG), ergosterol, and phosphatidylinositol phosphates (PtdInsPs), which have been discussed in recent review articles (Wickner and Rizo, 2017; Langemeyer et al., 2018; Starr and Fratti, 2019; Ungermann and Kümmel, 2019). The specific lipid composition of cellular membranes is recognized as a key factor in the multitude of essential biological processes performed in or on these membranes (Harayama and Riezman, 2018). The complex lipid composition of cellular membranes has been suggested to be a driving force behind the formation of regions of phase separation and lateral heterogeneities known as “lipid rafts,” whose biological significance is only just beginning to be understood (Sezgin et al., 2017). While there are detailed molecular mechanisms that describe glycerophospholipids as regulatory lipids in homotypic fusion, there is a lack of such research focusing on the role that sphingolipids play in this process, even though some species of these lipids were found to be enriched in endosomal and lysosomal fractions in earlier studies (Hechtberger et al., 1994). It has become abundantly clear that sphingolipids play a large role in lysosomal function and homeostasis in humans, providing ample reason to investigate the molecular mechanism(s) for sphingolipid-based regulation of lysosomal processes in other models (Kihara, 2016; Hannun and Obeid, 2018). In this review we highlight research that has focused on this subject and discuss outstanding questions and future perspectives related to it.

Sphingolipids in Membrane Trafficking and Endosomal Maturation

Membrane trafficking and maturation events have been extremely well-studied using the yeast system as a model over the past 40 years, and many of the pathways and effectors have been identified and investigated at varying levels (Feyder et al., 2015). Defects in vesicular trafficking have been identified in a number of studies concerning yeast impaired for sphingolipid synthesis and turnover. The yeast ortholog of human neutral sphingomyelinase type 2, Isc1p, catalyzes the removal of the headgroup sugars from glycosylated sphingolipids. Yeast that lack Isc1p are unable to degrade complex sphingolipids, causing a buildup of mannose-inositol-phosphoceramide (MIPC) and M(IP)2C, as well as altered levels of the second messenger long chain bases (LCBs) and LCB-1-phosphates (Sawai et al., 2000; Barbosa et al., 2011). These yeast also produce more non-hydroxylated C26-ceramide species, and less α-OH-phytoceramide species, presumably from an increase in de novo ceramide synthesis (Barbosa et al., 2011). In isc1Δ yeast, lysosomal trafficking is significantly altered, evidenced by the secretion of vacuole-destined carboxypeptidase Y (CPY/Prc1p) into the extracellular space, which could not be rescued by overexpression of Vam3p or Ykt6p and was attributed to increased ceramide activated protein phosphatase (CAPP) activity (Teixeira et al., 2016). Such a large increase in non-hydroxylated ceramide species as seen in the studies referenced above could have a thickening effect on cellular membranes, reducing the lateral mobility and fluidity of the bilayer and preventing the proper organization of effectors necessary for maturation and fusion. Defects in ceramide homeostasis and subsequent downstream signaling events were also detected in yeast with a temperature sensitive SEC14 allele and those that lack the endosomal SNARE Tlg2p (Mousley et al., 2008). The block in endosomal maturation resulted in widespread changes to the sphingolipid profile of these strains. The vacuolar SNAREs that promote the docking step of fusion were improperly trafficked when sphingolipid synthesis was disrupted by depletion of the acyl-CoA-binding protein Acb1p, and vacuoles from these strains were unable to fuse (Faergeman et al., 2004). Furthermore, work with the fission yeast S. pombe highlighted a role for MIPC in the trafficking of proteins to the plasma membrane and proper vacuole homeostasis (Nakase et al., 2010). These studies demonstrate the intimate ties between endosomal maturation and sphingolipid biosynthesis and turnover in yeast.

Endosomal maturation is a complex process that intertwines anterograde trafficking from trans-Golgi network (TGN) derived vesicles with endocytosed material from the cell’s exterior, ultimately to be degraded, recycled and/or sent to different organelles (Huotari and Helenius, 2011). By utilizing HPLC and advanced mass spectrometry techniques it was discovered that wild-type yeast sphingolipids have much less variation in acyl chain length and saturation compared to mammalian sphingolipids, almost exclusively requiring a saturated C26 very long chain fatty acid (VLCFA) bound via amide link to a LCB (Lester et al., 1993; Ejsing et al., 2006, 2009; Megyeri et al., 2016). This C26 VLCFA requirement is reinforced by the lethality of attempting to knockout ELO2 (formerly FEN1) and ELO3 (formerly SUR4) simultaneously (Revardel et al., 1995). These membrane-embedded, ER-localized proteins catalyze the first step of microsomal VLCFA elongation through the condensation of a long chain fatty acid with a malonyl-CoA unit (Denic and Weissman, 2007). A high-temperature suppressor screen revealed that increased expression of the endosomal Rab GTPase Vps21p could rescue the growth defect observed in elo3Δ yeast, and elo3Δvps21Δ, elo3Δvps3Δ, elo3Δvps19Δ, and elo3Δvps8Δ strains had significantly impaired growth rates (Obara et al., 2013). The proteins Vps3p/Vps8p are subunits of the CORVET endosomal-tethering complex, and Vps19p (Vac1p/Pep7p) is a PtdIns3P binding protein that functions in many steps of membrane trafficking (Weisman and Wickner, 1992; Webb et al., 1997; Plemel et al., 2011). The authors observed a similar genetic interaction by creating a csg1Δcsh1Δvps21Δ triple mutant strain, which blocked de novo synthesis of MIPC instead of disrupting VLCFA production. This reinforced the idea that the endosomal maturation process is dependent on C26-sphingolipids and the endosomal fusion machinery. The elo3Δvps21Δ yeast also showed abnormal proteolytic and glycosylation/maturation profiles for CPY, Pep4p (Proteinase A), Pho8p (alkaline phosphatase), and Cps1p (carboxypeptidase S/CPS). The Snc family of SNARE proteins participates in exocytic, endocytic, and recycling processes, and their function is regulated by complex sphingolipids, VLCFAs, and LCB-1-phosphates (David et al., 1998; Grote et al., 2000; Tani and Kuge, 2012). Taken together, these studies strongly suggest that sphingolipids play an active role in the membrane maturation events at endosomes and lysosomes in yeast.

Ergosterol and Raft Domains

The vertex ring domain that forms between docked vacuoles is enriched in proteins and lipids that are necessary for fusion, including ergosterol (Wang et al., 2002; Fratti et al., 2004; Karunakaran et al., 2012). Ergosterol has also been shown to be necessary for the activation of Cdc42p at the vacuole, promoting homotypic fusion that coincides with, but is not dependent on, Sec18p/Sec17p priming activity (Jones et al., 2010). Although it was shown that ergosterol production was necessary for activation, it’s unknown if this is due to physical interactions between GTPase and sterol, lipid raft modulation, or even through modulating the activity of a guanine nucleotide exchange factor (GEF) or GTPase activating protein (GAP) for Rho proteins at the vacuole.

Ergosterol and sphingolipids in yeast are key players in the lipid raft hypothesis. Liquid phase separation of lipids into stable micrometer domains was observed in giant unilamellar vesicles (GUVs) when monitoring the temperature- and lipid composition-dependent distribution of a fluorescent lipid-based dye (Veatch and Keller, 2003). These coexisting liquid phases were determined to be a liquid-disordered (Ld) like phase consisting of unsaturated acyl-chain phospholipids and a Lo like phase composed of saturated acyl-chain phospholipids and cholesterol. Therefore, it wasn’t entirely surprising that the same phenomenon could also be observed with GUVs made from isolated yeast PtdInsPs (containing an unsaturated acyl chain), ergosterol, and inositol-phosphoceramide (IPC; saturated acyl chains) (Klose et al., 2010). This study utilized Laurdan spectroscopy experiments to measure the anisotropy and movement of the dye within the membrane, and the results suggested that the formation of these domains depended on the presence of C26-phytosphingolipid species due their disappearance from GUVs when the lipids were isolated from elo3Δ or sur2Δ yeast. Some legitimate criticisms and questions about the presence of these membrane microdomains arose from their seemingly short lifetimes in vivo, invasive techniques for isolation and microscopic observation, and physiological relevance of phase transition temperatures. However, many of these questions were addressed when micrometer-scale membrane domains were visualized in live yeast for the first time with relatively non-invasive visualization techniques (Toulmay and Prinz, 2013). This study showed that selected vacuolar proteins with a fluorescent tag could segregate into one of two distinct and separate domains when yeast cells are grown to stationary phase. This segregation could also be induced by glucose starvation, translation inhibition via cyclohexamide, or mild acidic stress, indicating they likely have biological relevance in vacuole homeostasis. Interestingly, two proteins highlighted in this study, Vph1p (discussed below) and Ivy1p, have known and putative roles in the homotypic vacuole fusion cascade, respectively. Ivy1p is a possible I-BAR protein with a role in sensing membrane curvature for fusion and/or fission processes, and is known to interact with the Rab GTPase Ypt7p and the HOPS subunit Vps33p, both of which are necessary for the tethering step of vacuole fusion (Lazar et al., 2002; Numrich et al., 2015; Itoh et al., 2016). Ivy1p was shown to colocalize with the macrolide filipin III that binds to ergosterol in yeast vacuoles, indicating that Ivy1p resides in Lo like rafts enriched in ergosterol and sphingolipids following domain formation in the vacuole membrane. A cursory investigation of the proteins that were found to reside in the Ld like domain in the seminal study revealed that they all contain multiple transmembrane helices. Contrary to this, the proteins that localized to the Lo like domains are soluble proteins that interact with the vacuole membrane via larger membrane complexes (Gtr2p tethers to the membrane via the EGO complex, and Ivy1p binds to Ypt7p and HOPS complex), implying there may yet be a correlation between a protein’s structural biology and its residential membrane domain, but this will require in-depth studies. A screen for yeast mutants that were unable to produce these lipid raft domains in vacuoles pointed to genes in phospholipid production (NEM1 and FAB1) and endosomal maturation/multivesicular body (MVB) formation (VPS4) (Toulmay and Prinz, 2013). There have been some recent advances in understanding how these domains may form in the vacuolar membrane. Tsuji and colleagues showed that the yeast Niemann-Pick type C (NPC) orthologs Ncr1p and Npc2p are essential components for the creation and growth of the Lo ergosterol rich domain (Tsuji et al., 2017). This study also highlighted that that MVB pathway at the endosome facilitates ergosterol transport to the vacuole, again highlighting the interconnectivity of membrane trafficking and homeostasis mechanisms in yeast.

V-ATPase Function and Localization

The vacuolar ATPase (V-ATPase) is required for proper acidification of the organelle, which is necessary for the activation of resident hydrolases and autophagy, and Vph1p (V0 subunit) forms trans-complexes between vacuoles that promote homotypic fusion, and interacts with a number of fusion effectors (Nakamura et al., 1997; Peters et al., 2001). It was also shown that the localization of Vph1p can shift to the boundary under alkaline conditions for turnover via intralumenal fragment (ILF) recycling (McNally et al., 2017). Studies have linked the activity of the V-ATPase to sphingolipid levels in the vacuole membrane. It was discovered that isc1Δ yeast are unable to acidify the vacuole, and this was due to increased Sit4p-mediated CAPP activity (Teixeira et al., 2016). The V1 component of the V-ATPase requires VLCFAs for proper activity and is regulated by Orm1/2p controlled serine-palmitoyl transferase activity (Chung et al., 2003; Finnigan et al., 2011). Conversely, it was shown that the loss of individual V-ATPase components can drastically alter the levels of complex sphingolipids and hydroxylated species, indicative of a functional relationship between these lipids and vacuolar acidification (Tani and Toume, 2015). As previously mentioned, Vph1p was shown to segregate into a specific membrane compartment that is separate and distinct from the Lo like region enriched in Ivy1p and ergosterol (Toulmay and Prinz, 2013). This Vph1p-containing region was determined to be Ld like in nature due to an observed colocalization with the marker dye Fast DiI. The proton translocation activity is modulated via the regulatory lipid phosphatidylinositol 3,5-bisphosphate (PtdIns(3,5)P2), which would historically correlate well with a Ld membrane domain (Li et al., 2014; Banerjee et al., 2019). There is at least one study that challenges the model of PtdIns(3,5)P2 distributing to the Ld like region and suggests a pool may also enrich in the Lo like membrane rafts. This research used a quick-freezing and freeze-fracture replica labeling (QF-FRL) electron microscopy (EM) method coupled with a highly specific PtdIns(3,5)P2 binding probe to show that a large fraction of this lipid in the vacuole localizes to Ivy1p-enriched/Vph1p-depleted region following hyperosmotic stress (Takatori et al., 2016). This could suggest that there is a pool of PtdIns(3,5)P2 that is remodeled or synthesized with saturated acyl chains, and that membrane microdomains can be induced by distinct mechanisms possibly leading to multiple raft species with distinct lipid and protein compositions.

It is tempting to relate the location of Vph1p and Ivy1p membrane domains to the location and topography of the fusion machinery between tethered and docked vacuoles. We know that ergosterol, Ypt7p, and the HOPS complex localize to the vertex region during fusion, and Vph1p is normally mostly found ubiquitously throughout the vacuole membrane (Wang et al., 2002; Fratti et al., 2004; McNally et al., 2017). It is possible that the vertex region enriched in ergosterol is another Lo like microdomain, which may even form with a different lipid/protein composition than those identified above (Figure 1). Vacuoles are constantly undergoing fission and fusion events when cells are early in their chronological lifespan, which implies the membrane microdomains that only form after reaching stationary phase when vesicular trafficking has decreased would likely have less impact on the vacuolar fission/fusion process. We now know that lipid raft domains can form in the vacuole following a number of stress inputs (reviewed in Tsuji and Fujimoto, 2018), and it will require diligent work to piece together the contributing pathways and factors for the formation different domains. It would be interesting to see if the observable phase separation of vacuole membrane regions can persist following isolation on floatation gradients, and whether it can be induced with changes in pH or osmotic pressure.

FIGURE 1.

FIGURE 1

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The vertex domains of docked vacuoles may represent another lipid raft species. Left, Two-dimensional representation of docked vacuoles. Upon docking vacuoles form distinct morphological regions. The boundary membrane is the flattened area of apposed membranes. The vertex domains form at the transition between the boundary and outer undocked membranes. Right, A zoomed in view of the vertex-boundary transition area. The membranes are composed of disordered and ordered membrane raft-like microdomains. The disordered regions are composed of generalized phospholipids (e.g., phosphatidylcholine) in gray. The vertex domain is a raft-like domain shown as being thicker and contains sphingolipids (SL, pink), ergosterol (Erg, green), phosphoinositides (PtdIns, blue), and vertex-localized phospholipids (PL, mocha). The vertex domain contains SNAREs, Cdc42, Ypt7 and recruits the HOPS complex and is a site for actin polymerization. The V-ATPase subunit Vph1 is present in the ordered and disordered regions of the membrane, but fully assembled and functional V-ATPase requires de novo sphingolipid synthesis (not shown).

Autophagy

The vacuole is necessary for the highly conserved and essential autophagy degradation pathway that delivers cytoplasmic components for hydrolysis and recycling. This process is highly regulated by a number of mechanisms, including nutrient levels and target of rapamycin complex 1 (TORC1) activity at the vacuole (Reggiori and Ungermann, 2017). It was found that this process is also intimately tied to sphingolipids as autophagic flux and aminopeptidase I (Ape1p) processing are defective in isc1Δ yeast, and this could be rescued by downregulating the TORC1-Sch9p pathway (Teixeira et al., 2016). It is notable that the TORC1 stimulating GTPase Gtr2p of the vacuolar EGO complex localized to Lo like membrane rafts, adding another possible layer of autophagic communication between sphingolipid-rich lipid rafts and TORC1 signaling (Toulmay and Prinz, 2013). It was also shown that blocking endosomal maturation could lead to altered sphingolipid homeostasis and increased ceramide levels, which was found to block the unfolded protein response (UPR) at the ER and TORC1 activity, and these effects were again tied to Sit4p CAPP activity (Mousley et al., 2008). When yeast reach stationary phase they produce more lipid droplets (LDs) presumably to maintain lipid homeostasis within the cell (Walther and Farese, 2012). Wang and colleagues showed that the Lo like raft domains in the vacuole mediate the autophagy of these organelles (lipophagy), and this is dependent on a subset of canonical autophagy related genes (Atg) (Wang et al., 2014). Together these studies confirm the presence of a complicated relationship between sphingolipid metabolism and autophagy whose intricacies remain to be completely understood.

Conclusion and Future Perspectives

Most sphingolipid biosynthetic genes display varying levels of interactions with genes annotated as having a function in membrane trafficking and endolysosomal maturation. According to the Saccharomyces Genome Database1 AUR1 (the catalytic subunit to IPC synthase) displays genetic interactions with ATG1, GYP1, PEP1, SEC17, VAM7, VPH1, VPS4, VPS8, VPS9, VPS13, VPS21, VPS41, and VPS55. Future studies will require clever and well-planned in vitro and in vivo studies to understand the full contribution of sphingolipids and lipid rafts in the fusion cascade. Although complex sphingolipids are likely to be trafficked to the vacuole within the lumenal leaflet because their biosynthetic enzymes are housed in the lumen of the Golgi, ceramide may face either leaflet due to it higher rate of bilayer translocation or flip-flop, and there may be yet unknown or non-canonical transfer methods to move sphingolipids between leaflets (Levine et al., 2000; Sato et al., 2009). Alternatively, it is possible that the C26 VLCFA facilitates clustering across leaflets, as has been shown for GPI-linked proteins at the plasma membrane (Raghupathy et al., 2015). It would be ideal to create reconstituted systems to examine the sphingolipid contribution to the fusion mechanism, such as those done with SNAREs and proteoliposomes (Zick et al., 2014). Reconstituted in vitro systems will require careful isolation and purification of yeast sphingolipids due to a lack of commercial availability, but they will allow for tight control of the system to observe the direct contribution of individual sphingolipids to membrane fusion. It is likely that both Lo and Ld like membrane domains play a role in vacuole fusion, with each being enriched in different regulatory lipids and proteins that promote fusion. This is supported by the observation that the vertex ring domains are not homogeneous in nature and show a distribution of known fusion factors (Wang et al., 2002; Fratti et al., 2004; Wickner, 2010). There is also a desire for a sensitive sphingolipid-binding probe similar to the fluorescently tagged PtdInsP-binding domains that helped researchers determine the localization of PtdInsPs in a living cell (Burd and Emr, 1998; Várnai and Balla, 1998). Yeast will produce C6-NBD-IPC from C6-NBD-ceramide, but they won’t modify it further. This indicates that either substrate recognition for subsequent glycosylation enzymes heavily relies on the presence of a VLCFA bound at the amide position, or the presence of the fluorescent group prevents association with a substrate-binding pocket, and a similar phenomenon has been observed in some mammalian systems (Lipsky and Pagano, 1985; Levine et al., 2000).

While there is much left to discover, studies that focused on understanding the composition and biological relevance of lipid raft domains at the yeast vacuole have provided exciting results. Future studies should strive for technical coverage by utilizing a number of established methods in conjunction. These studies will need to seamlessly mix the cell biology and physical biochemistry of the membrane by using techniques such as mass spectrometry, Laurdan anisotropy, genetic manipulation, and advanced microscopy to name a few. While many studies referenced above use some of these techniques, further advancement in the field will require more thoughtful and advanced in vitro and in vivo techniques to overcome limitations and obtain a complete picture detailing how the lipid and protein composition of the yeast vacuole changes following stresses and upon reaching stationary phase, and the homeostatic pathways that communicate with this dynamic organelle.

Author Contributions

LH and RF conceived and wrote the manuscript. All authors contributed to the article and approved the submitted version.

Conflict of Interest

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

Funding. This work was supported by the National Science Foundation under award number MCB-1818310 to RF.

References

  1. Banerjee S., Clapp K., Tarsio M., Kane P. M. (2019). Interaction of the late endo-lysosomal lipid PI(3,5)P2 with the Vph1 isoform of yeast V-ATPase increases its activity and cellular stress tolerance. J. Biol. Chem. 294 9161–9171. 10.1074/jbc.ra119.008552 [DOI] [PMC free article] [PubMed] [Google Scholar]
  2. Barbosa A. D., Osório H., Sims K. J., Almeida T., Alves M., Bielawski J., et al. (2011). Role for Sit4p-dependent mitochondrial dysfunction in mediating the shortened chronological lifespan and oxidative stress sensitivity of Isc1p-deficient cells. Mol. Microbiol. 81 515–527. 10.1111/j.1365-2958.2011.07714.x [DOI] [PMC free article] [PubMed] [Google Scholar]
  3. Burd C. G., Emr S. D. (1998). Phosphatidylinositol(3)-phosphate signaling mediated by specific binding to RING FYVE domains. Mol. Cell 2 157–162. 10.1016/s1097-2765(00)80125-2 [DOI] [PubMed] [Google Scholar]
  4. Chung J. H., Lester R. L., Dickson R. C. (2003). Sphingolipid requirement for generation of a functional v1 component of the vacuolar ATPase. J. Biol. Chem. 278 28872–28881. 10.1074/jbc.m300943200 [DOI] [PubMed] [Google Scholar]
  5. David D., Sundarababu S., Gerst J. E. (1998). Involvement of long chain fatty acid elongation in the trafficking of secretory vesicles in yeast. J. Cell Biol. 143 1167–1182. 10.1083/jcb.143.5.1167 [DOI] [PMC free article] [PubMed] [Google Scholar]
  6. Denic V., Weissman J. S. (2007). A molecular caliper mechanism for determining very long-chain fatty acid length. Cell 130 663–677. 10.1016/j.cell.2007.06.031 [DOI] [PubMed] [Google Scholar]
  7. Ejsing C. S., Moehring T., Bahr U., Duchoslav E., Karas M., Simons K., et al. (2006). Collision-induced dissociation pathways of yeast sphingolipids and their molecular profiling in total lipid extracts: a study by quadrupole TOF and linear ion trap-orbitrap mass spectrometry. J. Mass Spectrom. 41 372–389. 10.1002/jms.997 [DOI] [PubMed] [Google Scholar]
  8. Ejsing C. S., Sampaio J. L., Surendranath V., Duchoslav E., Ekroos K., Klemm R. W., et al. (2009). Global analysis of the yeast lipidome by quantitative shotgun mass spectrometry. Proc. Natl. Acad. Sci. U.S.A. 106 2136–2141. 10.1073/pnas.0811700106 [DOI] [PMC free article] [PubMed] [Google Scholar]
  9. Faergeman N. J., Feddersen S., Christiansen J. K., Larsen M. K., Schneiter R., Ungermann C., et al. (2004). Acyl-CoA-binding protein, Acb1p, is required for normal vacuole function and ceramide synthesis in Saccharomyces cerevisiae. Biochem. J. 380 907–918. 10.1042/bj20031949 [DOI] [PMC free article] [PubMed] [Google Scholar]
  10. Feyder S., De Craene J. O., Bär S., Bertazzi D. L., Friant S. (2015). Membrane trafficking in the yeast Saccharomyces cerevisiae model. Int. J. Mol. Sci. 16 1509–1525. 10.3390/ijms16011509 [DOI] [PMC free article] [PubMed] [Google Scholar]
  11. Finnigan G. C., Ryan M., Stevens T. H. (2011). A genome-wide enhancer screen implicates sphingolipid composition in vacuolar ATPase function in Saccharomyces cerevisiae. Genetics 187 771–783. 10.1534/genetics.110.125567 [DOI] [PMC free article] [PubMed] [Google Scholar]
  12. Fratti R. A., Jun Y., Merz A. J., Margolis N., Wickner W. (2004). Interdependent assembly of specific regulatory lipids and membrane fusion proteins into the vertex ring domain of docked vacuoles. J. Cell Biol. 167 1087–1098. 10.1083/jcb.200409068 [DOI] [PMC free article] [PubMed] [Google Scholar]
  13. Grote E., Vlacich G., Pypaert M., Novick P. J. (2000). A snc1 endocytosis mutant: phenotypic analysis and suppression by overproduction of dihydrosphingosine phosphate lyase. Mol. Biol. Cell 11 4051–4065. 10.1091/mbc.11.12.4051 [DOI] [PMC free article] [PubMed] [Google Scholar]
  14. Hannun Y. A., Obeid L. M. (2018). Sphingolipids and their metabolism in physiology and disease. Nat. Rev. Mol. Cell Biol. 19 175–191. 10.1038/nrm.2017.107 [DOI] [PMC free article] [PubMed] [Google Scholar]
  15. Harayama T., Riezman H. (2018). Understanding the diversity of membrane lipid composition. Nat. Rev. Mol. Cell Biol. 19 281–296. 10.1038/nrm.2017.138 [DOI] [PubMed] [Google Scholar]
  16. Hechtberger P., Zinser E., Saf R., Hummel K., Paltauf F., Daum G. (1994). Characterization, quantification and subcellular localization of inositol-containing sphingolipids of the yeast, Saccharomyces cerevisiae. Eur. J. Biochem. 225 641–649. 10.1111/j.1432-1033.1994.00641.x [DOI] [PubMed] [Google Scholar]
  17. Huotari J., Helenius A. (2011). Endosome maturation. EMBO J. 30 3481–3500. 10.1038/emboj.2011.286 [DOI] [PMC free article] [PubMed] [Google Scholar]
  18. Itoh Y., Kida K., Hanawa-Suetsugu K., Suetsugu S. (2016). Yeast Ivy1p is a putative I-BAR-domain protein with pH-sensitive filament forming ability in vitro. Cell Struct. Funct. 41 1–11. 10.1247/csf.15014 [DOI] [PubMed] [Google Scholar]
  19. Jones L., Tedrick K., Baier A., Logan M. R., Eitzen G. (2010). Cdc42p is activated during vacuole membrane fusion in a sterol-dependent subreaction of priming. J. Biol. Chem. 285 4298–4306. 10.1074/jbc.m109.074609 [DOI] [PMC free article] [PubMed] [Google Scholar]
  20. Karunakaran S., Sasser T., Rajalekshmi S., Fratti R. A. (2012). SNAREs, HOPS, and regulatory lipids control the dynamics of vacuolar actin during homotypic fusion. J. Cell Sci. 14 1683–1692. 10.1242/jcs.091900 [DOI] [PubMed] [Google Scholar]
  21. Kihara A. (2016). Synthesis and degradation pathways, functions, and pathology of ceramides and epidermal acylceramides. Prog. Lipid Res. 63 50–69. 10.1016/j.plipres.2016.04.001 [DOI] [PubMed] [Google Scholar]
  22. Klose C., Ejsing C. S., García-Sáez A. J., Kaiser H. J., Sampaio J. L., Surma M. A., et al. (2010). Yeast lipids can phase-separate into micrometer-scale membrane domains. J. Biol. Chem. 285 30224–30232. 10.1074/jbc.m110.123554 [DOI] [PMC free article] [PubMed] [Google Scholar]
  23. Langemeyer L., Fröhlich F., Ungermann C. (2018). Rab GTPase function in endosome and lysosome biogenesis. Trends Cell Biol. 28 957–970. 10.1016/j.tcb.2018.06.007 [DOI] [PubMed] [Google Scholar]
  24. Lazar T., Scheglmann D., Gallwitz D. (2002). A novel phospholipid-binding protein from the yeast Saccharomyces cerevisiae with dual binding specificities for the transport GTPase Ypt7p and the Sec1-related Vps33p. Eur. J. Cell Biol. 81 635–646. 10.1078/0171-9335-00290 [DOI] [PubMed] [Google Scholar]
  25. Lester R. L., Wells G. B., Oxford G., Dickson R. C. (1993). Mutant strains of Saccharomyces cerevisiae lacking sphingolipids synthesize novel inositol glycerophospholipids that mimic sphingolipid structures. J. Biol. Chem. 268 845–856. [PubMed] [Google Scholar]
  26. Levine T. P., Wiggins C. A., Munro S. (2000). Inositol phosphorylceramide synthase is located in the Golgi apparatus of Saccharomyces cerevisiae. Mol. Biol. Cell 11 2267–2281. 10.1091/mbc.11.7.2267 [DOI] [PMC free article] [PubMed] [Google Scholar]
  27. Li S. C., Diakov T. T., Xu T., Tarsio M., Zhu W., Couoh-Cardel S., et al. (2014). The signaling lipid PI(3,5)P2 stabilizes V1-V(o) sector interactions and activates the V-ATPase. Mol. Biol. Cell 25 1251–1262. 10.1091/mbc.e13-10-0563 [DOI] [PMC free article] [PubMed] [Google Scholar]
  28. Li S. C., Kane P. M. (2009). The yeast lysosome-like vacuole: endpoint and crossroads. Biochim. Biophys. Acta 1793 650–663. 10.1016/j.bbamcr.2008.08.003 [DOI] [PMC free article] [PubMed] [Google Scholar]
  29. Lipsky N. G., Pagano R. E. (1985). Intracellular translocation of fluorescent sphingolipids in cultured fibroblasts: endogenously synthesized sphingomyelin and glucocerebroside analogues pass through the Golgi apparatus en route to the plasma membrane. J. Cell Biol. 100 27–34. 10.1083/jcb.100.1.27 [DOI] [PMC free article] [PubMed] [Google Scholar]
  30. McNally E. K., Karim M. A., Brett C. L. (2017). Selective lysosomal transporter degradation by organelle membrane fusion. Dev. Cell 40 151–167. 10.1016/j.devcel.2016.11.024 [DOI] [PubMed] [Google Scholar]
  31. Megyeri M., Riezman H., Schuldiner M., Futerman A. H. (2016). Making sense of the yeast sphingolipid pathway. J. Mol. Biol. 428 4765–4775. 10.1016/j.jmb.2016.09.010 [DOI] [PubMed] [Google Scholar]
  32. Mousley C. J., Tyeryar K., Ile K. E., Schaaf G., Brost R. L., Boone C., et al. (2008). Trans-Golgi network and endosome dynamics connect ceramide homeostasis with regulation of the unfolded protein response and TOR signaling in yeast. Mol. Biol. Cell 19 4785–4803. 10.1091/mbc.e08-04-0426 [DOI] [PMC free article] [PubMed] [Google Scholar]
  33. Nakamura N., Matsuura A., Wada Y., Ohsumi Y. (1997). Acidification of vacuoles is required for autophagic degradation in the yeast, Saccharomyces cerevisiae. J. Biochem. 121 338–344. 10.1093/oxfordjournals.jbchem.a021592 [DOI] [PubMed] [Google Scholar]
  34. Nakase M., Tani M., Morita T., Kitamoto H. K., Kashiwazaki J., Nakamura T., et al. (2010). Mannosylinositol phosphorylceramide is a major sphingolipid component and is required for proper localization of plasma-membrane proteins in Schizosaccharomyces pombe. J. Cell Sci. 123 1578–1587. 10.1242/jcs.059139 [DOI] [PubMed] [Google Scholar]
  35. Numrich J., Péli-Gulli M. P., Arlt H., Sardu A., Griffith J., Levine T., et al. (2015). The I-BAR protein Ivy1 is an effector of the Rab7 GTPase Ypt7 involved in vacuole membrane homeostasis. J. Cell Sci. 128 2278–2292. 10.1242/jcs.164905 [DOI] [PubMed] [Google Scholar]
  36. Obara K., Kojima R., Kihara A. (2013). Effects on vesicular transport pathways at the late endosome in cells with limited very long-chain fatty acids. J. Lipid Res. 54 831–842. 10.1194/jlr.m034678 [DOI] [PMC free article] [PubMed] [Google Scholar]
  37. Peters C., Bayer M. J., Buhler S., Andersen J. S., Mann M., Mayer A. (2001). Trans-complex formation by proteolipid channels in the terminal phase of membrane fusion. Nature 409 581–588. 10.1038/35054500 [DOI] [PubMed] [Google Scholar]
  38. Platt F. M., d’Azzo A., Davidson B. L., Neufeld E. F., Tifft C. J. (2018). Lysosomal storage diseases. Nat. Rev. Dis. Primers 4:27. [DOI] [PubMed] [Google Scholar]
  39. Plemel R. L., Lobingier B. T., Brett C. L., Angers C. G., Nickerson D. P., Paulsel A., et al. (2011). Subunit organization and Rab interactions of Vps-C protein complexes that control endolysosomal membrane traffic. Mol. Biol. Cell 22 1353–1363. 10.1091/mbc.e10-03-0260 [DOI] [PMC free article] [PubMed] [Google Scholar]
  40. Raghupathy R., Anilkumar A. A., Polley A., Singh P. P., Yadav M., Johnson C., et al. (2015). Transbilayer lipid interactions mediate nanoclustering of lipid-anchored proteins. Cell 161 581–594. 10.1016/j.cell.2015.03.048 [DOI] [PMC free article] [PubMed] [Google Scholar]
  41. Reggiori F., Ungermann C. (2017). Autophagosome maturation and fusion. J. Mol. Biol. 429 486–496. 10.1016/j.jmb.2017.01.002 [DOI] [PubMed] [Google Scholar]
  42. Revardel E., Bonneau M., Durrens P., Aigle M. (1995). Characterization of a new gene family developing pleiotropic phenotypes upon mutation in Saccharomyces cerevisiae. Biochim. Biophys. Acta 1263 261–265. 10.1016/0167-4781(95)00124-y [DOI] [PubMed] [Google Scholar]
  43. Sato K., Noda Y., Yoda K. (2009). Kei1: a novel subunit of inositolphosphorylceramide synthase, essential for its enzyme activity and Golgi localization. Mol. Biol. Cell 20 4444–4457. 10.1091/mbc.e09-03-0235 [DOI] [PMC free article] [PubMed] [Google Scholar]
  44. Sawai H., Okamoto Y., Luberto C., Mao C., Bielawska A., Domae N., et al. (2000). Identification of ISC1 (YER019w) as inositol phosphosphingolipid phospholipase C in Saccharomyces cerevisiae. J. Biol. Chem. 275 39793–39798. 10.1074/jbc.m007721200 [DOI] [PubMed] [Google Scholar]
  45. Sezgin E., Levental I., Mayor S., Eggeling C. (2017). The mystery of membrane organization: composition, regulation and roles of lipid rafts. Nat. Rev. Mol. Cell Biol. 18 361–374. 10.1038/nrm.2017.16 [DOI] [PMC free article] [PubMed] [Google Scholar]
  46. Starr M. L., Fratti R. A. (2019). The participation of regulatory lipids in vacuole homotypic fusion. Trends Biochem. Sci. 44 546–554. 10.1016/j.tibs.2018.12.003 [DOI] [PMC free article] [PubMed] [Google Scholar]
  47. Takatori S., Tatematsu T., Cheng J., Matsumoto J., Akano T., Fujimoto T. (2016). Phosphatidylinositol 3,5-Bisphosphate-rich membrane domains in endosomes and lysosomes. Traffic 17 154–167. 10.1111/tra.12346 [DOI] [PubMed] [Google Scholar]
  48. Tani M., Kuge O. (2012). Involvement of complex sphingolipids and phosphatidylserine in endosomal trafficking in yeast Saccharomyces cerevisiae. Mol. Microbiol. 86 1262–1280. 10.1111/mmi.12057 [DOI] [PubMed] [Google Scholar]
  49. Tani M., Toume M. (2015). Alteration of complex sphingolipid composition and its physiological significance in yeast Saccharomyces cerevisiae lacking vacuolar ATPase. Microbiology 161 2369–2383. 10.1099/mic.0.000187 [DOI] [PubMed] [Google Scholar]
  50. Teixeira V., Medeiros T. C., Vilaça R., Ferreira J., Moradas-Ferreira P., Costa V. (2016). Ceramide signaling targets the PP2A-like protein phosphatase Sit4p to impair vacuolar function, vesicular trafficking and autophagy in Isc1p deficient cells. Biochim. Biophys. Acta 1861 21–33. 10.1016/j.bbalip.2015.10.004 [DOI] [PubMed] [Google Scholar]
  51. Toulmay A., Prinz W. A. (2013). Direct imaging reveals stable, micrometer-scale lipid domains that segregate proteins in live cells. J. Cell Biol. 202 35–44. 10.1083/jcb.201301039 [DOI] [PMC free article] [PubMed] [Google Scholar]
  52. Tsuji T., Fujimoto M., Tatematsu T., Cheng J., Orii M., Takatori S., et al. (2017). Niemann-Pick type C proteins promote microautophagy by expanding raft-like membrane domains in the yeast vacuole. eLife 6:e25960. [DOI] [PMC free article] [PubMed] [Google Scholar]
  53. Tsuji T., Fujimoto T. (2018). Lipids and lipid domains of the yeast vacuole. Biochem. Soc. Trans. 46 1047–1054. 10.1042/bst20180120 [DOI] [PubMed] [Google Scholar]
  54. Ungermann C., Kümmel D. (2019). Structure of membrane tethers and their role in fusion. Traffic 20 479–490. 10.1111/tra.12655 [DOI] [PubMed] [Google Scholar]
  55. Várnai P., Balla T. (1998). Visualization of phosphoinositides that bind pleckstrin homology domains: calcium- and agonist-induced dynamic changes and relationship to myo-[3H]inositol-labeled phosphoinositide pools. J. Cell Biol. 143 501–510. 10.1083/jcb.143.2.501 [DOI] [PMC free article] [PubMed] [Google Scholar]
  56. Veatch S. L., Keller S. L. (2003). Separation of liquid phases in giant vesicles of ternary mixtures of phospholipids and cholesterol. Biophys. J. 85 3074–3083. 10.1016/s0006-3495(03)74726-2 [DOI] [PMC free article] [PubMed] [Google Scholar]
  57. Walther T. C., Farese R. V. (2012). Lipid droplets and cellular lipid metabolism. Annu. Rev. Biochem. 81 687–714. 10.1146/annurev-biochem-061009-102430 [DOI] [PMC free article] [PubMed] [Google Scholar]
  58. Wang C. W., Miao Y. H., Chang Y. S. (2014). A sterol-enriched vacuolar microdomain mediates stationary phase lipophagy in budding yeast. J. Cell Biol. 206 357–366. 10.1083/jcb.201404115 [DOI] [PMC free article] [PubMed] [Google Scholar]
  59. Wang L., Seeley E. S., Wickner W., Merz A. J. (2002). Vacuole fusion at a ring of vertex docking sites leaves membrane fragments within the organelle. Cell 108 357–369. 10.1016/s0092-8674(02)00632-3 [DOI] [PubMed] [Google Scholar]
  60. Webb G. C., Zhang J., Garlow S. J., Wesp A., Riezman H., Jones E. W. (1997). Pep7p provides a novel protein that functions in vesicle-mediated transport between the yeast Golgi and endosome. Mol. Biol. Cell 8 871–895. 10.1091/mbc.8.5.871 [DOI] [PMC free article] [PubMed] [Google Scholar]
  61. Weisman L. S., Wickner W. (1992). Molecular characterization of VAC1, a gene required for vacuole inheritance and vacuole protein sorting. J. Biol. Chem. 267 618–623. [PubMed] [Google Scholar]
  62. Wickner W. (2010). Membrane fusion: five lipids, four SNAREs, three chaperones, two nucleotides, and a Rab, all dancing in a ring on yeast vacuoles. Annu. Rev. Cell Dev. Biol. 26 115–136. 10.1146/annurev-cellbio-100109-104131 [DOI] [PubMed] [Google Scholar]
  63. Wickner W., Rizo J. (2017). A cascade of multiple proteins and lipids catalyzes membrane fusion. Mol. Biol. Cell 28 707–711. 10.1091/mbc.e16-07-0517 [DOI] [PMC free article] [PubMed] [Google Scholar]
  64. Zick M., Stroupe C., Orr A., Douville D., Wickner W. T. (2014). Membranes linked by trans-SNARE complexes require lipids prone to non-bilayer structure for progression to fusion. eLife 3:e01879. [DOI] [PMC free article] [PubMed] [Google Scholar]

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