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VAC14 nucleates a protein complex essential for the acute interconversion of PI3P and PI(3,5)P2 in yeast and mouse

Natsuko Jin, Clement Y Chow, Li Liu, Sergey N Zolov, Roderick Bronson, Muriel Davisson, Jason L Petersen, Yanling Zhang, Sujin Park, Jason E Duex, Daniel Goldowitz, Miriam H Meisler, Lois S Weisman

Author Affiliations

  1. Natsuko Jin1,,
  2. Clement Y Chow2,,
  3. Li Liu3,
  4. Sergey N Zolov1,
  5. Roderick Bronson4,
  6. Muriel Davisson5,
  7. Jason L Petersen1,
  8. Yanling Zhang1,
  9. Sujin Park1,
  10. Jason E Duex1,
  11. Daniel Goldowitz6,
  12. Miriam H Meisler*,2 and
  13. Lois S Weisman*,1
  1. 1 Department of Cell and Developmental Biology and Life Sciences Institute, University of Michigan, Ann Arbor, MI, USA
  2. 2 Department of Human Genetics, University of Michigan, Ann Arbor, MI, USA
  3. 3 Department of Anatomy and Neurobiology, University of Tennessee Health Science Center, Memphis, TN, USA
  4. 4 Department of Pathology, Harvard Medical School, Boston, MA, USA
  5. 5 Mutant Resources Program, The Jackson Laboratory, Bar Harbor, ME, USA
  6. 6 Department of Medical Genetics, University of British Columbia, Vancouver, BC, USA
  1. *Corresponding authors: Life Sciences Institute, 210 Washtenaw Avenue, Room 6437, The University of Michigan, Ann Arbor, MI 48109‐2216, USA. Tel.: +734 647 2539; Fax: +734 615 5499; E-mail: lweisman{at}umich.edu or E-mail: meislerm{at}umich.edu
  1. These authors contributed equally to this work

Abstract

The signalling lipid PI(3,5)P2 is generated on endosomes and regulates retrograde traffic to the trans‐Golgi network. Physiological signals regulate rapid, transient changes in PI(3,5)P2 levels. Mutations that lower PI(3,5)P2 cause neurodegeneration in human patients and mice. The function of Vac14 in the regulation of PI(3,5)P2 was uncharacterized previously. Here, we predict that yeast and mammalian Vac14 are composed entirely of HEAT repeats and demonstrate that Vac14 exerts an effect as a scaffold for the PI(3,5)P2 regulatory complex by direct contact with the known regulators of PI(3,5)P2: Fig4, Fab1, Vac7 and Atg18. We also report that the mouse mutant ingls (infantile gliosis) results from a missense mutation in Vac14 that prevents the association of Vac14 with Fab1, generating a partial complex. Analysis of ingls and two additional mutants provides insight into the organization of the PI(3,5)P2 regulatory complex and indicates that Vac14 mediates three distinct mechanisms for the rapid interconversion of PI3P and PI(3,5)P2. Moreover, these studies show that the association of Fab1 with the complex is essential for viability in the mouse.

There is a Have you seen ...? (January 2009) associated with this Article.

Introduction

Phosphoinositide phosphate (PIP) lipids are transiently generated on the cytoplasmic face of selected intracellular membranes. Spatial localization of the lipid kinases and phosphatases that generate specific PIPs produces unique PIP tags on different membrane compartments (Matteis and Godi, 2004; Behnia and Munro, 2005; Bolis et al, 2007). PIPs function through recruitment of specific effector proteins, which in turn regulate ion channels, membrane fission and fusion, and formation of membrane tubules. PI(3,5)P2 is synthesized by phosphorylation of PI3P. Both PI3P and PI(3,5)P2 are generated in the endomembrane system, a heterogeneous system of membranes involved in traffic to and from the plasma membrane, the lysosome, and the Golgi (Di Paolo and De Camilli, 2006). PI(3,5)P2 is a minor PIP present at <0.1 and <0.05% of total PI lipids in yeast and mammalian cells, respectively, compared with the more typical values of 2.5 and 0.2% for PI3P (Bonangelino et al, 2002; Duex et al, 2006b; Zhang et al, 2007).

The dynamic interconversion of PI3P and PI(3,5)P2 is regulated by at least five proteins in yeast: the lipid kinase Fab1p, lipid phosphatase Fig4p, the Fab1p activator Vac7p, the Fab1p inhibitor Atg18p, and Vac14p, a protein required for the activity of both Fab1p and Fig4p (Bonangelino et al, 1997, 2002; Gary et al, 1998, 2002; Dove et al, 2002, 2004; Rudge et al, 2004; Duex et al, 2006a, 2006b; Efe et al, 2007). Homologues of Fab1p, Vac14p and Fig4p are found in all eukaryotes. In yeast, Vac14p, Fab1p and Fig4p are localized on the vacuole membrane (Bonangelino et al, 2002; Dove et al, 2004; Rudge et al, 2004; Duex et al, 2006a) and form a complex (Botelho et al, 2008). In mammalian cells, these proteins, also known as Fab1/PIKfyve/PIP5K3, Fig4/Sac3, and Vac14/ArPIKfyve, are located on early and late endosomes (Ikonomov et al, 2006; Rutherford et al, 2006). Association of the three mammalian proteins in cultured cells has been demonstrated by coimmunoprecipitation and cosedimentation (Sbrissa et al, 2007). Genetic analysis in yeast shows that Vac14p is required for Fab1p and Fig4p function (Bonangelino et al, 1997; Duex et al, 2006b), but the mechanism of this regulation is not known.

We recently described lethal null mutations of mammalian Vac14 and Fig4 that revealed the critical function of PI(3,5)P2 for neuronal survival. A null mutation of Fig4 in the pale tremor mouse results in the formation of vacuoles in the cell bodies of neurons of the central nervous system (CNS) and peripheral nervous system, with extensive degeneration of sensory neurons of the dorsal root ganglia (DRG) and juvenile lethality around the time of weaning (Chow et al, 2007). A null mutation of Vac14 results in perinatal lethality with extensive degeneration of DRG neurons (Zhang et al, 2007). The level of PI(3,5)P2 is reduced by approximately 50% in cultured fibroblasts from both mutants. The increased sensitivity of neurons to mutations causing PI(3,5)P2 deficiency could result from the high rate of membrane turnover required for maintenance of axonal and dendritic processes (Volpicelli‐Daley and De Camilli, 2007). Vacuoles that contain the late endosome/lysosome marker LAMP‐2 accumulate in cells deficient in Fig4, Vac14 or Fab1 (Ikonomov et al, 2006; Rutherford et al, 2006; Chow et al, 2007; Zhang et al, 2007), suggesting that failure to resolve late endosomal vesicles may be responsible for vacuole accumulation. Human patients who are compound heterozygotes for missense and null mutations of Fig4 are affected by Charcot–Marie–Tooth type 4J, a severe peripheral neuronopathy (Chow et al, 2007; Zhang et al, 2008).

The ingls mouse, a spontaneous neurological mutant with autosomal recessive inheritance, arose at the Jackson Laboratory in 1991 (Bronson et al, 2003). We now report that a missense mutation of a conserved leucine residue in Vac14 is the molecular defect in ingls. As the ingls mouse survives for up to 3 weeks after birth, postnatal phenotypes caused by defective Vac14 function could be characterized. Examination of the corresponding mutation in yeast vac14, combined with analysis of additional partially functional mutants of yeast vac14 and fab1, led to the determination that Vac14 nucleates the PI(3,5)P2 regulatory complex. The mutants led to the identification of specific regions of the Vac14 protein required for interaction with proteins in the complex. We also demonstrate that two additional regulators of the Fab1 kinase, Vac7p and Atg18p, reside within the complex. We find that formation of the complex is essential for the osmotic‐stress‐induced activation of Fab1. Analysis of the new vac14 and fab1 mutants provides insights into the organization of the PI(3,5)P2 regulatory complex and its crucial function in the mammalian nervous system.

Results

Phenotype of the ingls mouse

The spontaneous mutation ingls (infantile gliosis) arose on the DBA/2J strain background and has been maintained by 23 generations of backcrossing to strain C57BL/6J to generate the congenic line B6. ingls. Homozygous ingls mutants exhibit reduced body size and diluted pigmentation that can be recognized as early as postnatal day 3 (P3) (Figure 1A). By P14, the mice exhibit a tremor and impaired motor function (Supplementary video). The frequency of affected offspring born from crosses between heterozygous carriers is consistent with Mendelian expectation (29/140, P=0.24). However, the maximal survival for ingls/ingls homozygotes is 3 weeks, with continuous losses between P1 and P21. Histological analysis of the brain revealed greatly enlarged ventricles (Figure 1B, middle panel). Small areas with the appearance of spongiform degeneration are visible in several brain regions, including the thalamus, brain stem and cerebellar nucleus (Supplementary Figure S1A). This pattern resembles the more widespread degeneration in the Fig4‐null mouse (Chow et al, 2007). However, spinal motor neurons and sensory neurons in the DRG remain intact during the lifetime of the ingls mutant (Supplementary Figure S1B). Intense staining for glial fibrillary acidic protein (GFAP) is evident throughout the ingls brain, suggesting widespread astrogliosis (Figure 1C and Supplementary Figure S2A). GFAP is sufficiently increased to be detected by western blot of cortical extracts (Supplementary Figure S2B). Increased GFAP staining is evident as early as E14.5 (not shown).

Figure 1.

ingls is caused by the missense mutation Vac14–L156R. (A) ingls homozygous mice at postnatal day 14 (P14) display reduced body weight and diluted coat colour. ingls/Vac14 compound heterozygotes at P14 are similar in appearance. (B) Severe hydrocephalus and enlarged ventricles in ingls homozygote (P16) and ingls/Vac14 compound heterozygotes (P14) (H&E staining). (C) GFAP‐stained astrocytes in neonatal ingls‐ and Vac14‐null mice. (D) Sequence chromatogram from exon 4 of an ingls/+ heterozygote demonstrates the c467 T>G nucleotide substitution. (E) The ingls mutation changes leucine 156 to arginine. Leucine 156 is evolutionarily invariant from yeast to mammals. Dots indicate amino‐acid identity with human Vac14. (F) Western blot of Vac14 protein in brain extracts of wild‐type and ingls mice. Loading control, GAPDH. (G) Reduced levels of PI(3,5)P2 in cultured fibroblasts from ingls mice. (H, I) Rescue of vacuole formation by wild‐type human Vac14 cDNA. Primary fibroblasts from ingls mice transfected with the indicated plasmids. At 24 h, cells were fixed with 4% paraformaldehyde in PBS for 10 min, room temperature. (H). Fluorescent cells were scored for the presence of vacuoles. Mean±s.d. for three independent experiments, >100 cells per experiment. (I) Representative cells are shown; arrows mark transfected cells. Bar, 20 μm.

Genetic mapping of ingls

The ingls mutation was first mapped to an 18 Mb interval on distal mouse chromosome 8, between microsatellite markers D8Mit86 and D8Mit88, by genotyping 31 affected F2 offspring from a cross between DBA/2J.ingls/+ and C57BL/6J (Bronson et al, 2003). Genotyping additional markers on chromosome 8 reduced the nonrecombinant region to a 5.7 Mb interval with the following gene order: SNP1 (111.6 Mb)—1/62—ingls—1/62—D8Mit88 (117.3 Mb) (Supplementary Figure S3A). This nonrecombinant region contains 63 annotated genes (Mouse Build 37.2, www.ensembl.org).

Identification of a mutation in Vac14

The Vac14 gene spans the region between 113.1 and 113.2 Mb on chromosome 8, within the ingls nonrecombinant region. Based on similarities between the ingls phenotype and null mutations of Vac14 and Fig4 (Chow et al, 2007; Zhang et al, 2007), we tested Vac14 as a candidate gene for ingls.

The 19 exons of Vac14 were amplified from genomic DNA of an affected ingls homozygote and sequenced. Comparison with the wild‐type sequence from strain C57BL/6J (Build 37.2, www.genome.ucsc.edu) identified the nucleotide substitution c.467T>G in exon 4 (Figure 1D). Strain DBA/2J, the strain of origin of the ingls mutation, contains the wildtype residue (not shown). The T>G substitution destroys a SacI endonuclease site, which was used to genotype the Vac14ingls allele. The mutation results in substitution of an arginine residue for the evolutionarily invariant residue leucine 156 (Figure 1E). Western blot analysis of brain extracts revealed normal abundance of Vac14 protein in the mutant brain (Figure 1F).

Noncomplementation of ingls and a Vac14‐null allele

To confirm the causal function of the Vac14‐L156R mutation in the ingls phenotype, we assessed the ability of the Vac14ingls allele to complement the recessive lethality of the null allele Vac14βgeo (Vac14) (Zhang et al, 2007). Heterozygous ingls mice (Vac14+/ingls) were crossed with null heterozygotes (Vac14+/−). The Vac14ingls/− compound heterozygotes were born in the predicted Mendelian ratio of 25% but did not survive to weaning, showing that ingls is allelic with the null allele (Supplementary Figure S3B). The compound heterozygotes reproduced the phenotype of the ingls homozygote, with reduced body size and diluted pigmentation (Figure 1A), as well as enlarged ventricles (Figure 1B). The phenotypic similarity between Vac14ingls/− compound heterozygotes and ingls homozygotes, the failure of the ingls allele to rescue the null homozygote, and the mapping of ingls to an interval of chromosome 8 that includes Vac14, support the identification of Vac14‐L156R as the ingls mutation. The survival of the compound heterozygotes to P14, compared with the neonatal lethality of null homozygotes, shows that the Vac14L156R allele retains partial function.

Reduced levels of PI(3,5)P2 and vacuolization of cultured ingls fibroblasts

Levels of phosphoinositide lipids were assessed in cultured ingls fibroblasts. In wild‐type fibroblasts, PI(3,5)P2 comprised 0.04% of total PI. In mutant ingls fibroblasts, PI(3,5)P2 was reduced to 50% of normal, whereas the levels of PI3P, PI4P and PI(4,5)P2 were unaffected (Figure 1G).

There is accumulation of intracellular cytoplasmic vacuoles in the cultured fibroblasts from ingls mice (Figure 1I, bottom). The vacuolated appearance of the ingls fibroblasts is similar to the fibroblasts from Vac14‐ and Fig4‐null mice, indicating that the reduced level of PI(3,5)P2 is responsible for the similarity (Chow et al, 2007; Zhang et al, 2007). Transfection of a construct expressing a wild‐type human Vac14–mCit fusion protein reduced the frequency of vacuolized ingls fibroblasts from 20 to 5% (Figure 1H and 1I). Correction by wild‐type Vac14 shows that the Vac14–L156R mutation is responsible for the ingls cellular phenotype. The stability of the mutant protein in vivo indicates that the Vac14–L156R protein is functionally impaired.

Prediction that Vac14 is composed entirely of HEAT repeats places the L156R mutation in repeat 4

HEAT repeats contain two anti‐parallel helices connected by a short loop. These units often appear as a tandem series and provide surfaces for protein–protein interactions (Groves et al, 1999; Andrade et al, 2000). Previous analysis of the Vac14p sequence identified 1–3 HEAT repeats (Dove et al, 2002). As HEAT repeat sequences are degenerated, many bona fide repeats are not detected by motif detection programs.

Analysis of the Vac14 protein sequence with the repeat finding program REP set at a confidence threshold of Pθ<1e−6 (http://www.embl‐heidelberg.de/~andrade/papers/rep/search.html) (Andrade et al, 2000) predicted eight HEAT repeats in the Saccharomyces cerevisiae Vac14p sequence. One additional repeat was identified by REP in Drosophila melanogaster and Schizosaccharomyces pombe sequences and, by sequence similarity, was found in the S. cerevisiae sequence. A second analysis incorporated Vac14p sequences from 17 diverse species. Predicted HEAT repeats were defined by three criteria: (1) identification by REP in one or more species using no confidence threshold; (2) secondary structure prediction of two helices connected by a short loop; (3) alignment by visual inspection with HEAT repeat consensus sequences from the Pfam database. This analysis identified 21 potential HEAT repeats in S. cerevisiae Vac14p (Figure 2A). Many exhibit sequence similarity in all 17 species (not shown). Yeast Vac14p is thus most likely to contain a minimum of 9 HEAT repeats and as many as 21 repeats, which would comprise the entire protein. Analysis of human Vac14 predicted 17 repeats, 15 of which have homologues in S. cerevisiae Vac14p. The L156R mutation is located in helix B of HEAT repeat 4 (Figure 2A). A similar analysis accurately predicted the 50 HEAT repeats of TOR1 (Perry and Kleckner, 2003).

Figure 2.

Vac14 nucleates the Fab1 complex. (A) Vac14 contains 21 and 17 HEAT repeats in S. cerevisiae (top) and mammalian Vac14 (bottom), respectively. Identical colours indicate homologous repeats between S. cerevisiae and mammalian Vac14. Red asterisk and blue arrows indicate ingls and vac14‐2 mutations, respectively. Underlines: HEAT repeats identified by REP with a confidence threshold better than at Pθ<1e−6. (B) Yeast two‐hybrid test of human Vac14 (HsVac14) or human Vac14–L156R (HsVac14‐L>R), fused with the GAL4‐activation domain (AD), interaction with itself, residues 346–1134 of human Fab1 or full‐length Fig4, fused with the GAL4‐binding domain (BD). Plasmids were cotransformed into the yeast cells and transformants were plated onto the SC‐LEU‐TRP plate and replica‐plated onto SC‐LEU‐TRP (control) or SC‐LEU‐TRP‐ADE‐HIS plate (test). Plates were incubated at 24°C for 10 days. Growth on the test plate indicates protein–protein interaction. (C) Yeast two‐hybrid test of Gal4‐AD fused with yeast Vac14p tested with Gal4‐BD fused with either Fab1p, Fig4p, Vac7p, Atg18p or Vac14p. Transformants were plated onto SC‐LEU‐TRP and replica‐plated onto SC‐LEU‐TRP (control) or SC‐LEU‐TRP‐ADE‐HIS+3AT (test). Plates were incubated at 24°C for 7 days. (D) Schematic of interactions between Fab1 and Fab1 regulators. (E) Vac14p–Venus coprecipitated Vac7p. Wild‐type or VAC14–Venus cells were used. (F) Analysis on glycerol gradients (10–50%) indicate that Fab1p and regulators form a complex >670 kDa. Molecular weight markers bovine serum albumin, 66 kDa, and thyroglobulin, 670 kDa, run in an adjacent tube. Representative profile of two independent gradients. vac14Δ/fig4Δ/ATG18–Venus cells expressing pRS413–VAC14–V5 and pRS415–FIG4–Myc were used.

The L156R mutation disrupts Vac14 interaction with Fab1 but not Fig4

HEAT repeat proteins usually function as scaffolds with multiple binding partners (Groves et al, 1999; Andrade et al, 2000). The prediction that Vac14 may be composed entirely of HEAT repeats suggested that Vac14 may bind proteins that regulate PI(3,5)P2 levels. Previous sedimentation and coimmunoprecipitation analysis demonstrated that mammalian Vac14, Fab1, and Fig4 associate with each other (Sbrissa et al, 2007). We tested potential interactions using the yeast two‐hybrid test and found that human Vac14 interacts with Fab1 and Fig4 (Figure 2B). The ingls mutation, Vac14‐L156R, specifically disrupts the interaction between Vac14 and Fab1 but retains interaction with Fig4 (Figure 2B). A third interaction of yeast Vac14p is self‐association (Dove et al, 2002). We find that human Vac14 also interacts with itself and this interaction is unaffected by the Vac14–L156R mutation (Figure 2B). These data suggest that disruption of the interaction between Fab1 and Vac14 is the molecular basis for the ingls mutant phenotype.

Vac14p interacts with the known protein regulators of PI(3,5)P2

To determine whether Vac14p interacts with the other proteins known to regulate PI(3,5)P2 levels, we tested Vac7p and Atg18p, two additional regulators of yeast Fab1p. As Fab1p and Vac7p are large proteins, we performed a yeast two‐hybrid test with constructs that expressed overlapping peptides from conserved regions of Fab1p and Vac7p. We found that Fab1p peptide 538–1085 and Vac7p peptide 394–918 interacted with yeast Vac14p in the yeast two‐hybrid test (Figure 2C). Vac14p also interacts with full‐length constructs of Fig4p and Atg18p and with itself (Figure 2C).

To determine whether each protein colocalizes with Vac14p in vivo, we generated a chromosomal integrant of a Vac14p fusion construct containing the fluorescent tag RFP–mCherry. Consistent with the yeast two‐hybrid studies, Vac14p–mCherry colocalized on the vacuole membrane with GFP‐ or Venus‐tagged Fab1p, Fig4p, Vac7p, and Atg18p (Supplementary Figure S5).

Fab1 and its regulators reside within a large protein complex

Coimmunoprecitation experiments were performed to test the model that Vac14p nucleates a large complex (Figure 2D). Using the tagged proteins Vac14p–HA and Vac14p–V5, we found that immunoprecipitation with anti‐HA antibody coprecipitated Vac14p–V5 (Supplementary Figure S4A). Furthermore, Fab1p containing a C‐terminal tandem affinity purification (TAP) tag (Fab1–TAP) coprecipitated Vac14p–V5 (Supplementary Figure S4B). Moreover, immunoprecipitation of Vac14p coprecipitates Fig4p (Supplementary Figure S4C). In addition, precipitation of Fig4p coprecipitates Fab1p (Supplementary Figure S4D). These interactions were reported independently (Rudge et al, 2004; Botelho et al, 2008), and it was proposed that Fab1p, Vac14p, and Fig4p form a ternary complex (Botelho et al, 2008).

Immunoprecipitation of Vac14p–Venus also coprecipitates Vac7p (Figure 2E). These coprecipitation experiments demonstrate that Vac14p interacts with itself, Fab1p, Fig4p, and Vac7p. We did not observe coprecipitation of Atg18p with Vac14p, Fab1p‐TAP, or Vac7p (not shown).

To determine whether the proteins form a large complex, we used sedimentation analysis of detergent solubilized yeast cell lysates. When lysates were fractionated on a 10–50% glycerol gradient, Fab1 was distributed in two peaks (Figure 2F). The smaller peak, fraction 3, contained monomeric Fab1p (predicted molecular weight 257 kDa). The larger peak, fractions 6–8, contained Fab1p in a complex that sediments more slowly than the 670 kDa molecular weight standard in fractions 4 and 5. Although the predicted molecular weights of Vac7p, Fig4p, and Vac14p are 128, 101, and 99 kDa, respectively, significant proportions of these proteins comigrated with the large Fab1p complex: Vac7p, in fractions 6 and 7; Fig4p, in fractions 6–8; and Vac14p, in fractions 5–8. That the peak fractions for Fab1p, Vac7p, Fig4p, and Vac14p overlap but are not identical may be explained by the presence of a mixture of partial and complete complexes. For example, the ternary complex of Fab1p, Vac14p, and Fig4p is found exclusively on the membrane of the vacuole, whereas Vac14p and Fig4p associate with each other in the cytosol (Botelho et al, 2008).

Most of the Atg18p (55 kDa) behaved as a monomer (fractions 1 and 2), but some Atg18p comigrated with the complex (fractions 5–7), suggesting that this small fraction is also part of the complex. Alternatively, the Atg18 in fraction 6 could be trailing from the earlier fractions. However, note that the intensity of fraction 6 is the same as fraction 5. Genetic evidence (below) strongly suggests that a portion of Atg18p is part of the Vac14p complex. Atg18p has a second distinct function in autophagy and the large proportion of monomeric protein may be related to that function.

The above‐mentioned results are consistent with the model that Vac14p nucleates a large complex containing Fab1p, Fig4p, Vac7p, Vac14p, and possibly Atg18p. Rather than pursuing analysis of the complex through further biochemical investigations, we identified and characterized mutations that partially disrupt the complex as a means to determine the functional significance of complete and partial complexes, and also map the interacting domains.

Fab1p, Vac14p, and Fig4p are required to form the core PI(3,5)P2 regulatory complex

Fab1p does not interact with Fig4p in a yeast two‐hybrid test. However, Fab1p–TAP coprecipitates with Fig4p, suggesting that the two proteins could interact indirectly. Indeed, coprecipitation of Fig4p by Fab1p–TAP required the presence of Vac14p and did not occur in the vac14Δ strain (Supplementary Figure S4E). Unexpectedly, coprecipitation of Fab1p–TAP with Vac14p required the presence of Fig4p (Supplementary Figure S4F). These data indicate that Fab1p requires both Vac14p and Fig4p to form a ternary complex in vivo. Localization experiments indicate that formation of the ternary complex is required for normal localization of members of the complex to the vacuole membrane (Figure 3A and B). Note that in each mutant, vac14Δ, fig4Δ, and fab1Δ, there is mislocalization to the cytoplasm of significant amounts of the remaining members of the complex.

Figure 3.

The localization of Fab1p, Fig4p, and Vac14p to the vacuole membrane requires the presence of all three proteins. Cells labelled with FM4‐64 (red) to visualize the vacuole membrane. (A) Wild‐type strains with FAB1–3xGFP, FIG4–3xGFP, or VAC14–Venus integrated at the proper chromosomal locus. (B) FAB1–3xGFP or FIG4–3xGFP/vac14Δ cells, FAB1–3xGFP or VAC14–Venus/fig4Δ cells and FIG4–3xGFP or VAC14–Venus/fab1Δ cells.

Vac7p binds Vac14p in yeast two‐hybrid and coimmunoprecipitation experiments (Figure 2C and 2E). To determine whether Vac7p is required for formation of the Fab1p/Vac14p/Fig4p complex, we carried out coprecipitation experiments in vac7Δ cells. Interaction of Fab1p with Vac14p (Supplementary Figure S6A) and Fig4p (Supplementary Figure S6B) did not require Vac7p. Localization of Fig4p, Vac14p, and Fab1p to the vacuolar membrane was independent of Vac7p (Supplementary Figure S6C). Similarly, Vac7p localization to the vacuole membrane is independent of Vac14p and Fig4p (Supplementary Figure S6C). Although two‐hybrid studies support the proposal that Atg18p is part of the complex, this was not observed by coprecipitation. To further investigate the association of Atg18p with the complex, we examined the effects of Vac14p mutations (below).

The Vac14–ingls mutation disrupts interaction with yeast Fab1p, Vac7p, and Atg18p

To further examine the molecular consequences of the ingls Vac14–L156R mutation, we generated the equivalent yeast mutant, vac14–L149R. The L149R mutation is located in HEAT repeat 4 (Figure 4A) and does not reduce protein stability (Figure 4B). The vac14Δ mutant has grossly enlarged vacuoles compared with the smaller and multilobed wild‐type vacuoles (Figure 4C). When vac14–L149R is present as the sole copy of VAC14, vacuole size and morphology are intermediate between the multilobed wild‐type and the vac14Δ mutant, consistent with partial loss of function (Figure 4C).

Figure 4.

The vac14–L149R mutant is defective in its association with Fab1p. (A) Schematic of the vac14–L149R mutant. Red asterisk: mutation site. (B) vac14–L149R protein is stable. Cell lysates from a vac14Δ strain expressing pRS413–VAC14‐HA or pRS413–vac14–L149R–HA (L>R) analysed by western blot. Vac14p detected with anti‐HA antibody. Loading control: Pgk1. (C) vac14–L149R mutant retains partial function. Vacuoles in the vac14–L149R mutant are intermediate in size between vac14Δ and wild‐type vacuoles. Vacuoles visualized with FM4‐64 (red). vac14Δ strain transformed with pRS413–VAC14, pRS413–vac14–L149R (vac14‐L>R), or pRS413 (vector). (D) Yeast two‐hybrid test of Vac14p or vac14p–L149R interaction with itself, Fab1p, Fig4p, Vac7p, and Atg18p. Full‐length Vac14p or vac14p–L149R (vac14‐L>R) fused with Gal4‐AD and Gal4‐BD. Full‐length Fig4p; Atg18p; amino acids 394–918 of Vac7p, amino acids 538–1085 of Fab1p, fused with Gal4‐BD. Upper panel, SC‐LEU‐TRP (control); lower panel, SD‐LEU‐TRP‐ADE‐HIS+3AT (test). (E) Pull‐down of Fab1p–TAP coprecipitates wild‐type Vac14p, but not vac14p–L149R. Detergent‐solubilized extracts from a vac14Δ or vac14Δ/FAB1–TAP strain expressing pRS413–VAC14–HA (WT), or pRS413–vac14–L149R–HA (L>R). Vac14p but not vac14p–L149R binds Fab1p–TAP IgG beads. (F) Fab1p localization is defective in the vac14p–L149R mutant. A vac14Δ/FAB1–3XGFP strain transformed with pRS413–VAC14 or pRS413–vac14–L149R (vac14‐L>R). FM4‐64 (red), Fab1p–3xGFP (green). (G) The vac14–L149R mutant does not increase its levels of PI(3,5)P2 in response to hyperosmotic stress. vac14Δ cells expressing pRS413–VAC14 or pRS413–vac14–L149R were labelled with [3H]inositol for 16 h and exposed to 0.9 M NaCl for times indicated. Values are the percentage of total extracted [3H]PI. Error bars: s.d. (n=3).

In a yeast two‐hybrid test, vac14p–L149R was defective in binding Fab1p, Vac7p, and Atg18p, although retaining normal interaction with Fig4p and with itself (Figure 4D). vac14p–L149R also failed to coprecipitate with Fab1p–TAP (Figure 4E). In the presence of vac14p–L149R, Fab1p did not localize to the vacuole membrane (Figure 4F). Thus, HEAT repeat 4 is critical for the interaction between Vac14p and Fab1p and is required for the intracellular localization of Fab1p.

In contrast, vac14p–L149R did coprecipitate with Fig4p and with itself (Supplementary Figure S7), indicating that the Fig4p and Vac14p interaction domains are located in a different region of Vac14p from the L149 mutation.

To examine the effect of loss of Fab1p from the PI(3,5)P2 regulatory complex, we examined the in vivo levels of PI(3,5)P2. Under basal conditions, PI(3,5)P2 comprises approximately 0.04% of total PI lipid in the vac14Δ strain expressing wild‐type VAC14 from a plasmid. When cells are exposed to hyperosmotic stress, PI(3,5)P2 increases 10‐fold to approximately 0.5% of total PI lipid within 10 min, then decreases to 0.3% at 20 min, and to 0.09% at 30 min (Figure 4G, Supplementary Table S1). (The 10‐fold increase in this wild‐type strain compared with a more typical 20‐fold increase may be a consequence of the expression of VAC14 from a plasmid rather than from its chromosomal location.) In the vac14Δ strain expressing vac14–L149R, PI(3,5)P2 comprises 0.03% of the PI lipid under basal conditions and increases only two‐fold to 0.06% after 10 min of hyperosmotic stress. Thus, dissociation of Fab1p from the complex through loss of interaction between Vac14p and Fab1p results in defective activation of Fab1 lipid kinase activity in response to hyperosmotic shock. That the modest increase in PI(3,5)P2 is sustained for at least 30 min suggests that regulation of Fig4p lipid phosphatase activity may also be impaired by the loss of association of Fab1p and Vac14p.

The fab1‐2 mutant reveals that activation of Fab1p requires its association with the Vac14p complex

We sought to identify a mutation in Fab1p that disrupted its interaction with Vac14p, and found that the fab1‐2 mutant (Yamamoto et al, 1995) is specifically defective in this interaction. We sequenced the mutant fab1‐2, and identified a single missense mutation, G864E, in the CCT domain (Figure 5A). The mutant protein is stable in vivo (Figure 5B) and retains normal kinase activity in vitro (Supplementary Figure S8). The CCT domain of Fab1p shares homology with the GroEL and the CCT family of Hsp60 chaperones, suggesting that it could be involved in protein–protein interactions. The G864E mutation is located within Fab1p peptide 538–1085, which interacts with Vac14p in a yeast two‐hybrid test (Figure 2C and 5C). We therefore tested the effect of this mutation on the interaction between Fab1 and Vac14. In the yeast two‐hybrid test, fab1–G864E does not interact with VAC14 (Figure 5C). Wild‐type Fab1p coimmunoprecipitates with Vac14p–Venus, but the Fab1p–G864E mutant does not (Figure 5D). Thus, the G864E mutation disrupts interaction of Fab1p with Vac14p.

Figure 5.

Formation of a ternary complex of Fab1p, Vac14p, and Fig4p is required for Fab1p kinase activity in vivo. (A) Schematic of the fab1‐2 allele; purple asterisk, the G864E mutation. (B) Fab1‐2 protein is present at wild‐type levels. Cell lysates analysed by western blot analysis from fab1Δ cells expressing pRS416–FAB1 or pRS416–fab1‐2. Equal protein loaded. (C) VAC14 interacts with FAB1, but not fab1‐2. Yeast two‐hybrid test of FAB1 or fab1‐2 interaction with VAC14. Full‐length VAC14 fused with Gal4‐AD. FAB1 or fab1‐2, amino acids 538‐1085. fused with Gal4‐BD. Upper panel, SC‐LEU ‐TRP (control); lower panel, SC‐LEU‐TRP‐ADE‐HIS+3AT (test). Plates incubated at 24°C for 4 days. (DE) fab1‐2 does not form a complex with Vac14p and Fig4p. (D) Vac14p–Venus does not coprecipitate fab1‐2. pRS416–FAB1 or pRS416–fab1‐2 expressed in a fab1Δ/VAC14–Venus strain. (E) fig4p–3xGFP does not coprecipitate fab1‐2. pRS416–FAB1 or pRS416–fab1‐2 expressed in a fab1Δ/FIG4–3xGFP strain. (F) fab1‐2, Vac14p and Fig4p in a fab1‐2 mutant do not localize to the vacuole membrane. pRS416–FAB1–3xGFP or pRS416–fab1‐2–3xGFP expressed in fab1Δ, or fab1Δ/VAC14–Venus or fab1Δ/FIG4–3xGFP. Cells labelled with FM4‐64 (red). (G) The fab1‐2 mutant does not transiently increase its levels of PI(3,5)P2 in response to hyperosmotic stress. fab1Δ cells expressing pRS416–FAB1 or pRS416–fab1‐2 measured as described in Figure 4. Error bars: s.d. (n=3).

Fab1p coimmunoprecipitates with Fig4p–3XGFP (Figure 5E). However, the Fab1p–G864E mutant protein does not coprecipitate with Fig4p–3XGFP (Figure 5E). This further supports the model that interaction of Fab1p with Fig4p is dependent on interaction of Fab1p and Fig4p with Vac14p (Supplementary Figure S4E and F). These coprecipitation results are similar to those observed for fab1p–T1017I, another point mutation in the CCT domain (Botelho et al, 2008).

The fab1‐2 mutant protein fails to localize to the vacuole membrane (Figure 5F). Localizations of Vac14p–Venus and Fig4p–3xGFP to the vacuole membrane are also defective in the presence of fab1‐2 protein (Figure 5F). Formation of the ternary complex thus appears to be required for correct localization of each component.

To determine the importance of formation of the ternary complex for the hyperosmotic stress‐induced activation of Fab1p, we tested the effect of osmotic stress on PI(3,5)P2 levels in the fab1‐2 mutant. In the wild‐type strain, the basal levels of PI(3,5)P2, 0.05% of total PI lipid, increase 20‐fold to 1.15% within 10 min after hyperosmotic stress, then decrease to 0.32% at 20 min and 0.11% at 30 min (Figure 5G, Supplementary Table S1). In the fab1‐2 mutant, the basal levels of PI(3,5)P2, 0.033%, increased only two‐fold after 10 min, similar to the vac14–L149 mutant described above. These data support the conclusion that association with the complex is required for the hyperosmotic stress‐induced activation of Fab1p and for the physiological regulation of PI(3,5)P2 levels.

The vac14‐2 mutant disrupts interaction with Vac7p and Atg18p and results in defective activation and inhibition of Fab1p

Vac7p is a major activator of yeast Fab1p, and basal levels of PI(3,5)P2 are significantly reduced in a vac7Δ mutant, resulting in enlarged vacuoles (Bonangelino et al, 1997; Duex et al, 2006b). We screened for gain‐of‐function mutations of Vac14p that could rescue the low levels of PI(3,5)P2 and reduce the enlarged vacuoles in vac7Δ cells. Random PCR mutagenesis of VAC14 was performed and the mutants were transformed into a vac14Δ, vac7Δ strain. Mutants that restored growth at 37°C and partially corrected the enlarged vacuoles were isolated. When the strongest of these mutants, vac14‐2, was expressed in a vac14Δ strain, vacuole size was smaller than in wild‐type cells (Figure 6A), suggesting that PI(3,5)P2 level is increased in this mutant. Direct measurement demonstrated a two‐fold increase of the basal level of PI(3,5)P2 in the vac14‐2 mutant (Figure 6B, Supplementary Table S1). However, when the vac14‐2 mutant was treated with hyperosmotic stress, the level of PI(3,5)P2 increased only 1.7‐fold, compared with an 8‐fold increase in the wild‐type strain (Figure 6B). There was no change in the steady‐state level of vac14‐2 protein compared with wild type (Figure 6C). The abnormal regulation of PI(3,5)P2 thus appears to be caused by altered function of the vac14‐2 protein.

Figure 6.

Vac7p and Atg18p function through Vac14p. (A) vac14‐2 has smaller than normal vacuoles, consistent with elevated basal levels of PI(3,5)P2. vac14Δ cells expressing pRS416–VAC14 or pRS416–vac14‐2 labelled with FM4‐64. (B) vac14‐2 has higher basal levels of PI(3,5)P2, but does not elevate or turnover PI(3,5)P2 during osmotic stress. PI(3,5)P2 levels in vac14Δ cells expressing pRS416–VAC14 or pRS416–vac14‐2 measured as described in Figure 4. Error bars: s.d. (n=3). (C) vac14‐2 protein is present at wild‐type levels. Cell lysates analysed by western blot analysis from vac14Δ cells expressing pRS413–VAC14–HA (WT) or pRS413–vac14‐2–HA(14‐2). Pgk1p: loading control. (D) Vac14‐2 is defective in binding Vac7p and Atg18p. Yeast two‐hybrid test of VAC14 or vac14‐2, fused with Gal4‐AD, interaction with FAB1, FIG4, VAC7, ATG18, fused with Gal4‐BD. Upper panel, SC‐LEU‐TRP (control); lower panel: SC‐LEU‐TRP‐ADE‐HIS +3AT (test). Plates incubated at 24°C, 7 days. (E) Fab1p coprecipitates vac14‐2. Detergent‐solubilized extracts from a vac14Δ or vac14Δ/FAB1–TAP strain expressing pRS413–VAC14–HA (WT), or pRS413–vac14‐2–HA (14‐2). (F) Schematic of the vac14‐2 allele; blue arrows indicate the mutation sites.

In a yeast two‐hybrid test, vac14 ‐2 is specifically defective in interaction with Vac7p and Atg18p (Figure 6D). Interaction of vac14‐2 protein with Vac14p, Fig4p, and Fab1p is normal and formation of the ternary complex is unaffected. The vac14‐2 protein also coprecipitates Fab1p to the same extent as wild‐type Vac14p (Figure 6E).

vac14‐2 contains four mutations: H56Y, R61K, Q101R, and L329I (Figure 6F). Three of these mutations, H56, R61, and Q101, are located in HEAT repeat loops 2 and 3. These residues exhibit evolutionary conservation. Tested singly in a yeast two‐hybrid test, each mutation perturbed the interaction of Vac14p with Vac7p and Atg18p, without disrupting interaction with its other binding partners (not shown). Thus all three residues are important for Vac14p interaction with Vac7p and Atg18p. L329 alone had no effect on the interaction of Vac14p with its known binding partners (data not shown). These results indicate that HEAT repeats 2 and 3 directly contact Vac7p and Atg18p, but do not contact Fab1.

The elevation in basal levels of PI(3,5)P2 in the vac14‐2 mutant is consistent with the model that negative regulation of Fab1p by Atg18p requires binding of Atg18p to Vac14p. Whereas the yeast two‐hybrid test detected interaction of Atg18p with Vac14p, this was not observed in pull‐down experiments. Thus, it is informative that a mutation in Vac14p that interrupts its ability to interact with Atg18p also results in PI(3,5)P2 levels that are consistent with a partial release of Atg18p inhibition of Fab1p. The vac14‐2 mutant provides additional support for the hypothesis that Atg18p interacts with Vac14p.

The vac14‐2 defect in osmotic stress‐induced elevation of PI(3,5)P2 supports the model that Vac7p, a positive regulator of Fab1p, exert an effect through binding to Vac14p. The association of Vac7p with wild‐type Vac14p was demonstrated in the yeast two‐hybrid test and by coimmunoprecipitation (Figure 2C, E).

The Fig4p‐binding site on Vac14p is distinct from the Fab1p‐, Vac7p‐, and Atg18p‐binding sites

Fab1p and Vac7p bind near the N terminus of Vac14p. On the basis of the predicted HEAT motifs of Vac14p, we divided the protein into two overlapping constructs (Figure 7). HEAT repeats 1–10 interact with Fab1p and Vac7p but not with Fig4p. HEAT repeats 10–21 interact only with Fig4p. These results demonstrate that Fab1p and Vac7p bind to the N‐terminal half of Vac14p, whereas Fig4p binds to a distinct site in the C‐terminal half. Atg18p binds full‐length Vac14p but does not bind to either half of the molecule. On the basis of the vac14‐2 mutant, we predict that contact points for Atg18p include the intrarepeat loops of HEAT repeats 2 and 3.

Figure 7.

Yeast two‐hybrid analysis of the minimal region of Vac14p required for interaction with Fab1p, Fig4p, Vac7p, and Atg18p. Lines above the schematic indicate the minimal region of Vac14p required for binding with each protein. Full‐length VAC14 or truncated VAC14 was fused with Gal4‐AD. FAB1 encoding amino acids 538–1085, VAC7 encoding amino acids 394–918: full‐length ATG18 or FIG4 was fused with the BD. Lines below the schematic indicate the regions of Vac14p tested.

Discussion

Here, we present support for the model that Fab1, Vac14, and Fig4 form a ternary complex. While this article was in preparation, independent evidence for formation of this complex in yeast was reported (Botelho et al, 2008). Our present studies significantly extend those studies by our discovery that the complex is nucleated by Vac14. Moreover, analysis of the new, partially functional fab1 and vac14 mutants demonstrate that the yeast complex includes Vac7p, a positive regulator of Fab1p, and is most likely to include Atg18p, an inhibitor of Fab1p. We find that both Vac7p and Atg18p exert an effect through direct contact with Vac14p. Our analysis strongly suggests that the organization of the complex produces dynamic, stimulus‐induced changes in PI(3,5)P2, by three distinct mechanisms. First, the activator Vac7p and the inhibitor Atg18p bind to overlapping sites, close to the site of Fab1p. This arrangement could facilitate the rapid activation and inactivation of the Fab1p lipid kinase during hyperosmotic stress in yeast. Second, Fab1p and Fig4p bind simultaneously to nonoverlapping sites on Vac14p, bring them into close proximity, so that the lipid kinase and phosphatase share access to the same pools of PI3P and PI(3,5)P2. Third, the close proximity of Fab1p and Fig4p is also consistent with our earlier postulate that Fig4p may function as a protein phosphatase to activate Fab1p by dephosphorylation (Duex et al, 2006b).

Vac14 contains multiple HEAT repeats

The partial loss of function of Vac14 in the ingls mouse prompted us to evaluate the molecular function of this uncharacterized protein. Our bioinformatics analysis predicted that both the yeast and mammalian Vac14 proteins are composed entirely of HEAT repeats. Tandem HEAT repeats form a super‐helical structure that provides docking sites for other proteins. The most common protein–protein docking sites are the intrarepeat loops (Groves et al, 1999; Xing et al, 2006). Three point mutations in vac14‐2 that impair protein interaction are located in predicted intrarepeat loops, R61K and H56Y in HEAT 2 and Q101R in HEAT 3. The location in the intrarepeat loops of three, random independent mutations that alter protein interactions supports the prediction of the HEAT repeat structure of Vac14. Analysis of the vac14‐2 mutant also indicates that Vac7p and Atg18p bind overlapping sites that include the intrarepeat loops of HEAT repeats 2 and 3.

A second potential protein–protein interaction site is on a face formed by the B helices of HEAT repeats (Chook and Blobel, 1999; Cingolani et al, 1999). The helices provide both structure and points of protein–protein contact. The ingls mutation is located on the predicted B helix of HEAT 4. This mutation affects the binding of Fab1p and also impairs binding of Atg18p and Vac7p. The Fab1p‐, Atg18p‐, and Vac7p‐binding sites may overlap, or the vac14–L149R mutation may perturb the surrounding structure, altering the Fab1p‐binding site and a separate Atg18p/Vac7p‐binding site. The overlap of Atg18p and Vac7p sites at a position close to the Fab1p‐binding site is consistent with competitive regulation of Fab1p by its positive and negative regulators.

Vac14 is a scaffold for the Fab1 kinase complex

As HEAT repeats mediate protein–protein interactions, we investigated and found that Vac14p nucleates the assembly of a complex containing the proteins that synthesize and turn over PI(3,5)P2. The location of the vac14–L149R and vac14‐2 mutations near the N‐terminal region of Vac14p indicates that the N‐terminal half of Vac14p binds Fab1p, Vac7p, and Atg18p. Indeed, in a yeast two‐hybrid test, HEAT repeats 1–10 of Vac14p were sufficient to bind Fab1p and Vac7p (Figure 7). Conversely, HEAT repeats 10–21 of Vac14p were sufficient to bind Fig4p (Figure 7). Thus, Fab1p, Fig4p, and two additional Fab1p regulatory proteins all directly contact Vac14p and make a large complex that regulates both the synthesis and turnover of PI(3,5)P2.

The composition of the PI(3,5)P2 regulatory complex facilitates dynamic regulation of PI(3,5)P2

The fab1‐2 mutation disrupts the ability of Fab1p to interact with Vac14p and prevents coprecipitation of Fab1p with Fig4p. Negative two‐hybrid test results (not shown) suggest that Fab1p and Fig4p do not interact directly. Fab1p binds to the N terminus and Fig4p binds to the C terminus of Vac14p. We propose that Vac14p assumes a conformation that brings Fab1p into close proximity to Fig4p (Figure 8). This physical proximity may explain our previous evidence that the lipid phosphatase Fig4p is an activator of the Fab1p kinase, possibly through dephosphorylation of the Fab1 protein. Importantly, the phosphatase activity of Fig4p is required for its regulatory function; an active site mutant that retains interaction with Vac14p is nonetheless defective in elevation of PI(3,5)P2 levels (Bonangelino et al, 1997; Duex et al, 2006b). Fig4p may also contribute to Fab1p activation through stabilization of the regulatory complex.

Figure 8.

Model of the Vac14 complex. (A) Schematic Vac14. (B) Vac14p binds to both Fab1p and Fig4p and may undergo a conformational change that brings Fab1p into contact with Fig4p. Fig4p functions as both an activator of Fab1p and a PI(3,5)P2 5‐phosphatase. Fig4p and Fab1p bind to distinct regions on Vac14p. The Fab1p‐binding site significantly overlaps with Vac7p‐ and Atg18p‐binding sites. Blue arrowheads indicate the vac14‐2 mutations sites, the arrow to the left indicates the location of H56Y and R61K, the arrow to the right marks Q101R. These arrows show the region of Vac14p that contacts Vac7p and Atg18p. Red asterisk indicates the vac14‐ingls mutation, which disrupts interaction with Fab1p, Vac7p, and Atg18p.

In addition to both the lipid phosphatase and lipid kinase, the PI(3,5)P2 regulatory complex includes a second pair of proteins with opposing effects on PI(3,5)P2 levels: a lipid kinase activator and inhibitor. The close association of each of these proteins in a complex may be key to the rapid modulation of PI(3,5)P2 levels in vivo (Duex et al, 2006a).

Identification of the components of the Vac14p complex provides new insights into the acute regulation of PI(3,5)P2 levels. First, the Fab1p lipid kinase and Fig4p lipid phosphatase reside in the same complex and bind to opposite ends of Vac14p. A conformational change in Vac14p could simultaneously affect the activities of the kinase and phosphatase in opposite directions, amplifying the net effect on PI(3,5)P2. Second, the complex contains both an activator and an inhibitor of Fab1p, Vac7p, and Atg18p, respectively, which bind to the same region of Vac14p, and most likely bind close to Fab1p. Again, an altered conformation of Vac14p could result in opposite effects on binding of the two proteins, amplifying the effect of either one alone on Fab1p activity. Third, Fig4p has a dual function and is both a lipid phosphatase and an activator of the lipid kinase. The structure of the protein complex is most likely to facilitate the rapid flux in PI(3,5)P2 levels that occurs in response to various biological stimuli.

PI(3,5)P2 is required for neural function and pigmentation

Similar to the null mutations of mouse Fig4 and Vac14 (Chow et al, 2007; Zhang et al, 2007), the Vac14ingls mutation results in reduced intracellular levels of PI(3,5)P2, cytoplasmic vacuolization, neurodegeneration, and early lethality. As the Vac14‐null mouse dies perinatally, defects in nervous system function were inferred solely from the histopathology of newborn mice. The ingls mouse lives up to 3 weeks, permitting direct observation of abnormal neurological function, pigmentation, and growth defects. The Vac14–ingls mice develop a tremor and motor incoordination exemplified by ataxic gait and difficulty in righting. Although the steady‐state levels of Vac14–ingls protein are normal and interaction with Fig4 is retained, binding of Fab1 is abolished. The failure of the corresponding yeast mutant to activate Fab1 strongly suggests that failure of ingls Vac14–L156R to activate mammalian Fab1 accounts for the low level of PI(3,5)P2 in fibroblasts from the ingls mouse. The data suggest that dissociation of Fab1 from the PI(3,5)P2 regulatory complex is the molecular basis for neurodegeneration and lethality in the ingls mouse. Thus, the ability of Vac14 to nucleate the complete PI(3,5)P2 regulatory complex is essential for normal neural function.

Differences between the Vac14–ingls, Vac14‐null and Fig4‐null mice are listed in Supplementary Table S2. DRG neurons are severely affected in the Fig4‐ and Vac14‐null mice, but are spared in the Vac14ingls mutant. This rescue of sensory neurons may be explained by their greater capacity for synthesis of PI(3,5)P2, or by a higher abundance of downstream effector proteins. The Vac14–ingls mutant exhibits astrocytosis with earlier onset and greater severity than the other mutants, which merits further investigation. Hydrocephalus is also more severe in the ingls mice, with huge distention of the ventricles. Differences in the abundance of interacting proteins may account for the cell‐type‐specific effects of these mutations. The mixed‐strain backgrounds of the two null mutants may also contribute to phenotypic differences from the congenic C57BL/6J.ingls mice discussed here.

Defects of PI(3,5)P2 regulation and human disease

Mutations of human FIG4 result in the peripheral neuropathy Charcot–Marie–Tooth type 4J, with features similar to those in the Fig4‐null mouse (Chow et al, 2007). To determine whether mutations of Vac14 could contribute to Charcot–Marie–Tooth disorder, we screened the previously described cohort of 95 patients for variants of VAC14. No variants in coding sequence or splice sites of VAC14 were observed (C Chow, M Meisler, M Khajavi, K Szigeti and JR Lupski, unpublished data). We also investigated the function of VAC14 in the human neurological disorder SCA4, which maps to a region of chromosome 16q22 that contains the VAC14 gene (Flanigan et al, 1996). We sequenced the exons of VAC14 in an affected member of the original SCA4 family, but did not detect any coding or splice site mutations (C Chow, M Meisler, and Y‐H Fu, unpublished data). Thus, the contribution of VAC14 mutations to human disease remains unknown. Extensive gliosis in patients with Alexander disease is caused by mutation of GFAP; it is possible that VAC14 or FIG4 could contribute to other disorders characterized by gliosis. The lack of DRG defects in the ingls mice, in contrast to the previously described null mutants, suggests that VAC14 could have an important function in human neurological disorders that are restricted to the CNS and have not yet been tested.

Evolutionary conservation of PI(3,5)P2 regulation

Our study used the cognate mutation in yeast to provide molecular insight into the pathology of the ingls mouse. This work indicates that the activation of Fab1 by the Vac14 complex is conserved from yeast to mammals and is essential for nervous tissue function, pigmentation and viability. Vac14 nucleates assembly of the PI(3,5)P2 core regulatory complex in yeast and serves as a scaffold for the complex (Figure 8). Loss of interaction between Vac14 and Fab1 results in the lethal neurological disorder in ingls mice. Analysis of the ingls mutation enabled us to localize the Fab1‐interaction domain of Vac14. In yeast, the vac14–ingls mutation also disrupts interaction with Vac7p, a positive regulator of Fab1p, and Atg18p, a negative regulator. The mammalian homologue of Vac7p has not been identified, whereas four distinct homologues of Atg18p are present in the mammalian genome: WIPI 1–4. Further work will be required to identify all components of the mammalian PI(3,5)P2 regulatory complex and to determine the functions of PI(3,5)P2. Thus far, we have described pathological mutations in the core components Fig4 and Vac14 (Chow et al, 2007; Zhang et al, 2007; this article). Heterozygous mutations of human FAB1 cause the mild eye phenotype corneal fleck dystrophy (OMIM 609414). In view of the vulnerability of neurons to alteration of PI(3,5)P2 levels, mutations in other components of the PI(3,5)P2 regulatory complex are likely to contribute to human neurological disease.

Materials and methods

Animals

The ingls mutation arose at The Jackson Laboratory in 1991 on the inbred strain DBA/2J and is maintained as a congenic line on the C57BL/6J background (current generation F23). Mice are available from the Jackson laboratory as B6.D2‐ingls/J (stock 003095). Preliminary description of the mutant and its location on chromosome 8 was submitted to the Jackson Laboratory website (Bronson et al, 2003). The Vac14βgeo line was generated from a gene‐trap ES cell from strain 129/Ola, and it lacks detectable protein (Zhang et al, 2007). The gene‐trap mice were first crossed to strain C57BL/6J and the Vac14βgeo mutant has been maintained as a mixed stock (C57BL/6J X 129/Ola)F12, by mating heterozygotes.

Genotyping

SNP1, CTC AAA CTT CAC CCC (C/T) AGC CCC ACC CCA ACC, is located at nucleotide 111,611,180 of mouse chromosome 8 (Mouse Build 37.1, www.ensembl.org) and was genotyped at Kbiosciences (www.kbioscience.co.uk/software/snpviewer). Mouse Vac14 exon 4 containing the ingls mutation is amplified with the following primer pair, designated as Vac14E4: forward, 5′CAG CCA GTG GGA ACA ACC GTG TGA; and reverse, 5′ ACA TAG ACA TGC AAG CAG GCA AAG. These primers are used for genotyping the L156R mutation by virtue of the loss of a SacI site in the mutant allele (Figure 1B).

Histology

Tissues were sectioned and stained with H&E at HistoServ (Germantown, MD). For GFAP staining, mice were perfused with 4% paraformaldehyde, and tissues were sectioned and stained as described (Liu et al, 2007). Twenty‐micrometer cryostat sections were stained with anti‐GFAP (1:1000, rabbit polyclonal, Sigma) and with secondary antibodies conjugated with biotin (1:200, Vector Laboratory, Burlingame, CA) followed by avidin–biotin complex (1:50, Elite, Vector Laboratory). Immunoreactivity was visualized with diaminobenzidine and 0.02% hydrogen peroxide for up to 5 min.

Western blot

For mouse samples, dissected brain cortex was homogenized in 150 mM NaCl, 1.0% NP‐40, 0.5% deoxycholate, 0.1% SDS, 1 mM EDTA, 50 mM Tris–HCl, pH 8.0, with protease inhibitors; Roche (Cat. no. 11 873 580 001), and lysed on ice for 1 h. Molecular weight markers; Amersham (cat. no. RPN7567). Anti‐Vac14 antibody (Zhang et al, 2007). For yeast samples, experiments were performed as described previously (Duex et al, 2006b).

Phosphoinositides and vacuoles in cultured cells and yeast cells

For cultured cells, primary fibroblasts were starved in inositol‐free DMEM 12 h and labelled with myo‐[2‐3H]inositol, 36 h. Lipids were extracted, deacylated, and analysed by anion‐exchange HPLC chromatography (Zhang et al, 2007). Images of cells were taken on an Axioscope 2 (Carl Zeiss MicroImaging, Jena, Germany) using a LUCPlanFL N × 40/0.60 Ph2 objective with a DeltaVision microscope system. For yeast cells, experiments were performed as described previously (Duex et al, 2006b).

Prediction of HEAT repeat motifs

Seventeen Vac14 sequences analysed were from: S. cerevisiae (NP_013490.1); Ashbya gossypii ATCC 10895 (NP_984909); Aspergillus fumigatus Af293 (XP_751167.1); Kluyveromyces lactis (XP_454179.1); Yarrowia lipolytica (XP_501232.1); Gibberella zeae PH‐1 (XP_390022.1); Candida glabrata (XP_447078.1); Ustilago maydis 521(XP_757421.1); Candida albicans SC5314 (XP_716167.1); Neurospora crassa OR74A (XP_959537.1); Debaryomyces hansenii CBS767 (XP_456837.1); S. pombe 972 h (NP_596363.1); Cryptococcus var. neoformans B‐3501A (XP_775858.1); Homo sapiens (NP_060522.3); Caenorhabditis elegans (NP_492215); D. melanogaster (NP_650208); Arabidopsis thaliana (NP_565275). Potential HEAT repeats in each sequence are identified using REP without an applied confidence threshold. Regions of S. cerevisiae Vac14 with homology to the predicted HEAT repeat in other species were assumed to form HEAT repeats. The resulting repeats were further analysed by the secondary structure prediction program (http://www.bioinf.manchester.ac.uk/dbbrowser/bioactivity/NPS2.html). Regions predicted to form two helices connected with a loop were selected. This predicted 21 and 17 HEAT repeats in S. cerevisiae and human Vac14, respectively. We manually aligned the human Vac14 sequence with random seed sequences from the Pfam database and obtained the same 17 repeats.

Fluorescence microscopy

Yeast cells labelled with FM4‐64 (Duex et al, 2006a). Fluorescence and differential interference contrast (DIC) images generated with a Deltavision system (Applied Precision, WA). Images are processed using Adobe Photoshop.

Immunoprecipitation in yeast cells

A total of 10 OD log‐phase cells were lysed in lysis buffer; 50 mM Tris pH 7.5, 120 mM NaCl, 10 mM EDTA, 1 mM EGTA, 5 mM 2‐glycerophosphate, 1 mM PMSF, 10 mM benzamidine, 1 mg/ml leupeptin, 5 mg/ml aprotonin. Extracts were spun at 500 g to sediment unbroken cells. Octyl‐glucoside (Sigma) was added to the supernatant to a final concentration of 0.5%. Subsequent manipulations were performed at 4 °C. Resulting extracts were incubated for 30 min and spun at 13 000 g, 10 min. Anti‐HA (COVANCE), anti‐GFP (Roche Applied Science) or anti‐V5 (Invitrogen) were added to the supernatant and incubated for 1 h. Protein A immobilized on Sepharose beads (Sigma) was added and incubated for 1 h. Protein complexes bound to the beads were washed seven times with lysis buffer containing 0.5% octyl‐glucoside, then eluted in sample buffer (50 mM Tris, pH6.8, 2% SDS, 5% β‐mercaptoethanol, 10% glycerol, 0.01% BPB) at 80°C, 5 min. SDS–PAGE and western blot analysis were used to detect Vac14–HA or V5, Vac7, Fab1, Fig4–Myc.

Yeast two‐hybrid analysis

VAC14 was subcloned into the XmaI–SalI site of pGAD or pGBD. FAB1 encoding amino acids 538–1085 was subcloned into the EcoRI–BglII site of pGBD. VAC7 encoding amino acids 394–918 was subcloned into SmaI–SalI site of pGBD. ATG18 was subcloned into the EcoRI–SalI site of pGBD. FIG4 was subcloned into the BamHI–PstI site of pGBD. Plasmids were cotransformed into the yeast strain PJ69‐4A, transformants were plated onto SC‐LEU‐TRP, replica‐plated onto SC‐LEU‐TRP, SC‐LEU‐TRP‐ADE‐HIS+3AT, or SC‐LEU‐TRP‐ADE‐HIS and grown for 4–10 days at 24°C. The yeast strain PJ69‐4A and the pGAD and pGBD vectors have been described (James et al, 1996).

Glycerol gradients

A total of 12 ml of 10–50% glycerol gradients were prepared in the lysis buffer with 0.5% octyl‐glucoside. S13 lysates were prepared from 20 OD cells as described above, loaded on the top and spun at 31 000 r.p.m. for 18 h at 4°C. Fractions (1 ml) were precipitated with TCA, and 1/10 of the sample was separated by SDS–PAGE.

Supplementary data

Supplementary data are available at The EMBO Journal Online (http://www.embojournal.org).

Supplementary Information

Supplementary video [emboj2008248-sup-0001.mov]

Supplementary Information [emboj2008248-sup-0002.pdf]

Acknowledgements

We thank Dr Lucia Rameh for the protocol to generate the labelled lipid standards. We thank Drs Yui Jin, Rob Piper, Guy Lenk, Cole Ferguson, and members of the Weisman and Meisler labs for helpful discussions. We thank Emily Kauffman for technical assistance. This work was supported by NIH grants R01‐GM50403 to LSW, R01‐GM24872 to MHM, T32 GM07544 training grant to CYC, and RRO1183 to the Mouse Mutant Resource at the Jackson Laboratory.

References

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