NuA4 Lysine Acetyltransferase Complex Contributes to Phospholipid Homeostasis in Saccharomyces cerevisiae.

Actively proliferating cells constantly monitor and readjust their metabolic pathways to ensure the replenishment of phospholipids necessary for membrane biogenesis and intracellular trafficking. In Saccharomyces cerevisiae, multiple studies have suggested that the lysine acetyltransferase complex NuA4 plays a role in phospholipid homeostasis. For one, NuA4 mutants induce the expression of the inositol-3-phosphate synthase gene, INO1, which leads to excessive accumulation of inositol, a key metabolite used for phospholipid biosynthesis. Additionally, NuA4 mutants also display negative genetic interactions with sec14-1ts , a mutant of a lipid-binding gene responsible for phospholipid remodeling of the Golgi. Here, using a combination of genetics and transcriptional profiling, we explore the connections between NuA4, inositol, and Sec14 Surprisingly, we found that NuA4 mutants did not suppress but rather exacerbated the growth defects of sec14-1ts under inositol-depleted conditions. Transcriptome studies reveal that while loss of the NuA4 subunit EAF1 in sec14-1ts does derepress INO1 expression, it does not derepress all inositol/choline-responsive phospholipid genes, suggesting that the impact of Eaf1 on phospholipid homeostasis extends beyond inositol biosynthesis. In fact, we find that NuA4 mutants have impaired lipid droplet levels and through genetic and chemical approaches, we determine that the genetic interaction between sec14-1ts and NuA4 mutants potentially reflects a role for NuA4 in fatty acid biosynthesis. Altogether, our work identifies a new role for NuA4 in phospholipid homeostasis.

Cellular processes, such as proliferation and intracellular trafficking, depend on a vast network of proteins involved in regulating phospholipid metabolism (Figure 1). Membrane phospholipid composition is, in part, established by highly conserved families of lipid-binding proteins that, as their name suggests, bind cellular lipids to facilitate lipid transport, modulate enzymatic activity, and even regulate the transcription of metabolic genes (reviewed in Henry ; Olkkonen 2013; Jackson and Bouvet 2014; Tripathi ). Phospholipid metabolism can also be fine-tuned by signaling pathways such as post-translational modifications. Indeed, it has recently emerged that lysine acetylation contributes to lipid metabolism by regulating both gene expression and the activity of metabolic enzymes (reviewed in Drazic ; Menzies ).

Figure 1

Overview of phospholipid metabolism. Key lipid metabolic proteins mentioned in the text are indicated, transcription factors/repressors are in circles, and lipids species are indicated in black rectangles. CDP-DAG, cytidine diphosphate diacylglycerol; PA, phosphatidic acid; PI, phosphatidylinositol; PI-4-P, phosphatidylinositol-4-phosphate; TAG, triacylglycerol; SE, steryl ester.

Several genome-wide genetic screens performed in Saccharomyces cerevisiae have revealed interactions between the highly conserved lysine acetyltransferase (KAT) complex NuA4 and phospholipid metabolic genes, suggesting a role for NuA4 in phospholipid homeostasis. NuA4 is a 13-subunit KAT complex containing the essential catalytic domain Esa1 (reviewed in Doyon and Cote 2004) and held together by the scaffolding protein Eaf1 (Auger ; Mitchell ). One role for NuA4 is the regulation of chromatin remodeling and gene transcription through the acetylation of histones H4 and H2A-Z (reviewed in Lu ), and growing evidence indicates that NuA4 also targets nonhistone proteins (reviewed in Downey and Baetz 2016).

Interestingly, several functional genomic screens have determined that NuA4 subunit mutants display an excessive accumulation of inositol, also called an Opi- phenotype (Hancock ; Salas-Santiago and Lopes 2014). Opi1 is a lipid-binding protein that represses transcription of target genes including the inositol-3-phosphate synthase, , as well as other phospholipid metabolic genes containing inositol/choline-responsive elements (ICREs) within their promoters (Greenberg ; Hirsch and Henry 1986; White ). These genes are derepressed under inositol-depleted conditions through a mechanism involving the relocation of Opi1 from the nucleus to the endoplasmic reticulum, where it binds to phosphatidic acid (Loewen , 2004). Deleting leads to the overexpression of , which in turn causes an excessive accumulation of inositol, referred to as the Opi- phenotype (Greenberg ). High-throughput genomic screens have identified many other mutants that derepress transcription and cause excessive accumulation of inositol, including mutants of the NuA4 complex (, , , , , and ) (Hancock ; Salas-Santiago and Lopes 2014). Interestingly, despite binding to its promoter, NuA4 is not required for the transcriptional activation of (Suka ; Konarzewska ), suggesting that the Opi- phenotype of NuA4 mutants is due to an uncharacterized role for NuA4 in the regulation of ICRE-containing genes as well as phospholipid homeostasis. NuA4 subunit mutants are unique among Opi- mutants as they also negatively interact with a mutant of the phospholipid-remodeling protein Sec14, providing an opportunity to dissect the particular role of NuA4 in phospholipid metabolism.

Sec14 is an essential phospholipid-binding protein that coordinates the metabolism of phosphatidylinositol-4-phosphate (PI-4-P) with phosphatidylcholine (PC) at the Golgi to create a lipid environment necessary for trafficking events (reviewed in Ghosh and Bankaitis 2011). Sec14-deficient mutants cause multiple effects related to phospholipid metabolism, including increased intracellular PC (McGee ; Xie ) and decreased PI-4-P (Hama ; Li ; Schaaf ). However, Sec14-deficient mutants also exhibits growth defects under inositol-depleted conditions (Patton-Vogt ), which is associated with an inability to derepress expression leading to decreased inositol biosynthesis under conditions lacking an exogenous source of inositol (Culbertson and Henry 1975; Villa-Garcia ). Synthetic genetic screens identified a mutant of the NuA4 complex, Δ, as one of several mutants that display a growth defect in combination with the temperature-sensitive mutant () (Curwin ). A separate high-throughput synthetic dosage lethal screen found that overexpression of , a gene whose function directly antagonizes Sec14 by depleting PI-4-P (Fang ; LeBlanc and McMaster 2010; Alfaro ), resulted in decreased viability in the NuA4 mutants Δ and Δ, and lethality in Δ (Mitchell ).

The negative genetic interaction between and NuA4 mutants are unexpected as one might anticipate that overproduction of inositol (Opi- phenotype) of the NuA4 mutants would suppress the growth defect in cells. This dichotomy provides an elegant means to start dissecting the function of NuA4 within this pathway. Here, we report that deletion or mutation of NuA4 subunits increased the growth defect in cells under inositol-depleted conditions. Further investigation through the use of RNA sequencing (RNA-seq) of Δ cells revealed that although transcription of was significantly upregulated, the transcription of other ICRE-containing genes was not. This suggests that the role of NuA4 under inositol-depleted conditions extends beyond inositol biosynthesis, most likely through other aspects of phospholipid homeostasis. In fact, we find that NuA4 mutants have impaired lipid droplet levels, which implies defects in the biosynthesis of triacylglycerol (TAG) and steryl esters (SEs). Through genetic and chemical approaches, we determine that the genetic interaction between and NuA4 mutants potentially reflects a role for NuA4 in fatty acid biosynthesis. Altogether, our work identifies a role for NuA4 in phospholipid homeostasis through regulation of fatty acid synthesis and lipid droplets.

Materials and Methods

Yeast strains, plasmids, and media

All strains used in this study are in the BY4741 (S288C) background and are listed in Table 1. Strains were generated either by standard mating methods or a PCR-mediated gene insertion/deletion technique (Longtine ). Strains from the Deletion Mutant Array (DMA) collection (GE, catalog no. YSC1053) were confirmed by PCR. A tetracycline/doxycycline inducible promoter (ptet) was used for overexpression, as previously described (Roney ). All cells were grown in either standard YPD or SC media, as indicated. SC-inositol media was made by mixing 6.7 g/liter of YNB with ammonium sulfate, without inositol (Millipore, catalog no. 4027-412) with 2 g/liter of standard amino acid complete mix. Myo-inositol (Sigma, catalog no. I5125), doxycycline (Sigma, catalog no. D3447), choline chloride (Sigma, catalog no. C7017), or dH2O was added to media after autoclaving to the concentration desired. Plates containing cerulenin (Sigma, catalog no. C2389) also contained 1% Brij 58 detergent (Sigma, catalog no. P5884-100G) to help dissolve the drug.

Table 1

Strain list

Strain ID	Genotype	Source
YKB1079/BY4741	MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0	Brachmann et al. (1998)
YKB3333	MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0	DMA collection (GE)
	eaf1Δ::KANMX
YKB3144/CMY505	MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0	Fairn et al. (2007)
	sec14-1ts-NATMX
YKB3935	MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0	This study
	sec14-1ts-NATMX eaf1Δ::KANMX
YKB3292	MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0	DMA collection (GE)
	eaf7Δ::KANMX
YKB4068	MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0	This study
	sec14-1ts-NATMX eaf7Δ::KANMX
YKB4236	MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0	This study
	esa1Δ::HIS3 esa1-L254Pts-URA3
YKB4242	MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0	This study
	sec14-1ts-NATMX esa1Δ::HIS3 esa1-L254Pts-URA3
YKB4325	MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0	This study
	ade2Δ::ptet-CDS1-TAP-LEU2,HIS3
YKB4326	MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0	This study
	ade2Δ::ptet-CDS1-TAP-LEU2,HIS3 sec14-1ts-NATMX
YKB4327	MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0	This study
	ade2Δ::ptet-CDS1-TAP-LEU2,HIS3 eaf1Δ::KANMX
YKB4328	MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0	This study
	ade2Δ::ptet-CDS1-TAP::LEU2,HIS3 sec14-1ts-NATMX eaf1Δ::KANMX
YJP1078	MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0	Gaspar et al. (2011)
	dga1Δ::KANMX lro1Δ::KANMX are1Δ::KANMX are2Δ::KANMX
YKB4337	MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0	This study
	sec14-1ts-NATMX dga1Δ::KANMX lro1Δ::KANMX are1Δ::KANMX are2Δ::KANMX
YKB4338	MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0	This study
	eaf1Δ::URA3 dga1Δ::KANMX lro1Δ::KANMX are1Δ::KANMX are2Δ::KANMX
YKB4339	MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0	This study
	sec14-1ts-NATMX eaf1Δ:URA3 dga1Δ::KANMX lro1Δ::KANMX are1Δ::KANMX are2Δ::KANMX

Spot assays

Cultures were grown in YPD, SD, or SC –inositol (+75 µM myo-inositol) as indicated at 30° prior to being diluted to an OD600 of 0.1, and four times 10-fold serial dilutions (OD600 = 0.1, 0.01, 0.001, and 0.0001) were plated and incubated for 2 d at the indicated temperatures. Images of spot assays were taken with the Bio-Rad Chemidoc XRS system under EPI-white light illumination and on the autoexposure setting.

RNA-seq

The strains (CMY505) and Δ (YKB3935) were grown in triplicate in 50 ml of YPD at 30° to midlog growth phase (OD600 = 0.5), then shifted to prewarmed YPD media at 33.5° for 2 hr before harvesting, washing with dH2O, and flash-freezing on dry ice. Cells were subsequently lysed by resuspending pellets in 100 µl of lyticase reaction solution [1.2 M sorbitol (Sigma, catalog no. S1876); 1 mg/ml lyticase (Sigma, catalog no. SRE0018)] and incubated at 30° for 30 min. RNA was purified using the RNA mini-kit (Ambion, catalog no. 12183018A) following the manufacturer’s yeast extraction protocol. Purified RNA extracts were then twice treated with DNaseI (Promega, catalog no. M6101) for 1 h at 37° each time followed by a phenol/chloroform extraction. After two DNaseI treatments, purified RNA was resuspended in 30 µl of RNase-free water. Three micrograms of purified RNA spiked with 1.5 µg of ERCC RNA control (Ambion, catalog no. 4456740) was depleted of ribosomal RNA (rRNA) using the Ribo-Zero Gold rRNA depletion kit for yeast (Illumina, catalog no. MRZY1306) and resuspended in 10 µl of RNase-free water. Successful depletion of the 18S and 26S rRNA was confirmed using the Agilent Bioanalyzer RNA 6000 Pico quantification kit (Agilent Technologies, catalog no. 5067-1513).

Whole transcriptome RNA-seq libraries were prepared using the Ion Total RNA-Seq Kit V2 (Life Technologies, catalog no. 4479789) and the Ion-Xpress RNA-seq Barcode 1-16 kit (Life Technologies, catalog no. 4475485) according to the manufacturer’s recommendations, using 50 ng of input rRNA depleted total RNA. The size distribution and yield of the final barcoded RNA-seq libraries was assessed using the Agilent Bioanalyzer High Sensitivity DNA quantification kit (Agilent Technologies, catalog no. 5067-4626). All six RNA-seq libraries were multiplexed and sequenced on the Life Technologies Ion Torrent Proton platform using a single Ion Proton Chip.

Resulting reads were aligned against the S. cerevisiae S288c genome (version GCF_000146045.2_R64) using the TMAP aligner provided with the Torrent Suite (v5.0.4). Raw sequencing reads have been deposited at the NCBI SRA archive under accession number PRJNA350552. Variation in sample processing during rRNA depletions and library construction was assessed using the ERCC analysis plugin (v5.0.0.0). The number of reads aligning to each annotated transcript was determined using bedtools (v2.17.0) (Quinlan and Hall 2010). Differential expression of transcripts between and Δ was determined using DESeq2 (v1.10.1) (Love ). Transcripts with a fold change of two or more and an adjusted p value ≤0.05 were considered to be differentially expressed. Gene ontology term analysis of enriched biological processes was conducted by using the DAVID bioinformatic online database (https://david.ncifcrf.gov) (Huang da et al. 2009). Significantly downregulated or upregulated genes were clustered into functionally related groups using the Gene Functional Classification Tool. The highest ranking Biological Process term was subsequently assigned for each group.

qRT-PCR

RNA extracts were prepared as above but without rRNA depletion. Purified RNA (2 µg) was reverse transcribed using the High Capacity cDNA Reverse Transcriptase Kit (Applied Biosciences, catalog no. 4368814) and resulting cDNA was diluted 1:10 for qRT-PCR. Transcript levels were measured using the SsoFast EvaGreen Supermix for qPCR (Bio-Rad, catalog no. 172-5201) with the Bio-Rad MiniOpticon Real-Time PCR system and CFX manager software. Primers used for qRT-PCR are as follows: (1) forward (Forw) primer: 5′-TCTCTGTTGCCCATGGTTAG-3′ and reverse (Rev) primer: 5′-CTTCAAGCGTTGTTGCAGAT-3′; (2) Forw: 5′-TGAAGGTGTTCCATCTCCAA-3′ and Rev: 5′-CGACTAGATTCTT-CGCACCA-3′; Forw: 5′-GCCAGAACAAGATGGGAAAT-3′ and Rev: 5′-TGTATGGACGACCCTTCAAA-3′; Forw: 5′-GCCATGGTGGTATCACAGAC-3′ and Rev: 5′-TCTGCTTGTCGTTCAGGTTC-3′; Forw: 5′-TTCTCAGGGCACTACACAGG-3′ and Rev: 5′-AAGGGACCAGGATACACTGC-3′; Forw: 5′-TGATTAATATGCCACCGGAA-3′ and Rev: 5′-ATGTTTGTCATCGCCAAGTG-3′; Forw: 5′-CTGTCAAGTTGAACAAGGAAACCAC-3′ and Rev: 5′-CAACGTGTTCAACCAAGTCGACAA-3′; Forw: 5′-GCCTTCTACGTTTCCATCCA-3′ and Rev: 5′-CGTAAATTGGAACGACGTGA-3′. A standard curve was constructed using a five times fivefold serial dilution series of pooled cDNA sample from the original individual reverse transcription reactions starting at a 1:5 dilution. The geometric averaging of two internal reference genes, and , was used for normalization of relative expression levels (Pfaffl 2001) using the Bio-Rad CFX Manager software. Three biological and two technical replicates were used for each sample. Statistical analyses were completed using a two-tailed unpaired t-test (p ≤ 0.05) with the GraphPad Prism software.

Immunoblotting

Samples were grown in SC media at 30° until midlog growth phase (OD600 = 0.5–0.6), then shifted to SC media with indicated amounts of doxycycline for 4 hr, before being harvested by centrifugation, washed in water, aliquoted in 1.5-ml Eppendorf tubes, and flash frozen in liquid nitrogen. Pellets were resuspended in 30% TCA lysis buffer and lysed mechanically by vortex with glass beads. Cell debris and glass beads were removed by centrifugation. Whole cell extract (WCE) was diluted in Laemmli loading dye and stored at −80°. The prepared samples were boiled at 95° for 10 min prior to separation by SDS-PAGE on a linear SDS-polyacrylamide gel (7.5%). Western blotting was performed using a semidry transfer apparatus from Bio-Rad (Trans-Blot SD Semi Dry Electrophoretic Transfer Cell; catalog no. 170-3940). Blocking, primary, and secondary incubations were performed with 5% milk in TBS-T (0.1% Tween 20; VWR, catalog no. CA95017-122L). Primary incubations were carried out at 4° overnight with rabbit α-TAP antibodies (1:10,000 dilution; Thermo Fisher, catalog no. PICAB1001) and secondary incubations at room temperature for 1 hr with peroxidase-conjugated goat α-rabbit IgG (1:10,000 dilution; Chemicon, catalog no. AP307P). Chemiluminescence was detected using Immobilon Western Chemiluminescent HRP substrate (Millipore, catalog no. WBKLS0500) and developed on a ChemiDoc XRS system (Bio-Rad, catalog no. 170-8070).

Lipid droplet

Cultures were grown in SC-inositol (+75 µM myo-inositol) media at 30° to midlog growth phase (OD600 = 0.5), washed in dH2O, and transferred to SC-inositol media supplemented with or without 75 µM of myo-inositol and grown for 2 hr at 30°. Cells were subsequently incubated with 10 µM BODIPY 493/503 (Life Technologies, catalog no. D3922) for 10 min at room temperature in their residing media and washed with dH2O. Cells were pelleted, resuspended in SC-inositol media (+ or − inositol), and loaded onto prewashed microscope slide with coverslips. Images were taken using the CellVoyager CV1000 disk confocal microscope (Yokogawa Electric Corporation, Musashino Tokyo, Japan). Brightfield (20% intensity, 100-ms exposure time, 100% gain) and BODIPY fluorescence, using FITC filters (25% intensity, 50-ms exposure time, 20% gain), were taken across multiple fields of view to capture at least 100 cells on the 100× oil immersion objective. Images for each field of view were taken at 0.2-µm steps for a total of 30 images. Image analysis was done using a custom MATLAB script. Bright field images were first thresholded using an adaptive thresholding algorithm. The resulting thresholded images were segmented using our MATLAB script that incorporated previously published code (Ricicova ), as well as our own code that makes use of functions found in the MATLAB Image Processing Toolbox. The cell outlines obtained through segmentation were used to quantify the area (in pixels) and total fluorescence from the fluorescence images. Fluorescence was quantified using the middle z-stack for each cell. Fluorescence density was calculated by dividing total fluorescence by area. A total of three biological replicates with >100 cells were analyzed for each sample. Mean fluorescence for each sample are converted relatively to wild-type samples in inositol-supplemented conditions. Statistical analyses were performed by one-way ANOVA with the Tukey’s multiple comparisons test, using the GraphPad Prism software.

Data availability

Strains and code are available upon request. Supplemental Material, File S1 contains the complete RNA-seq data set and gene functional classification analysis. Raw sequencing reads have been deposited at the NCBI SRA archive under accession number PRJNA350552.

Results

NuA4 mutants exacerbate the growth defects of sec14-1ts under inositol-depleted conditions

The growth defects of on inositol-depleted media can be suppressed by mutants which exhibit an overproduction of inositol phenotype (Opi-) due to the derepression and transcription of the rate-limiting biosynthetic enzyme within this pathway, (Patton-Vogt ; Chang ). As NuA4 mutants exhibit a derepression of and excessive inositol production, or Opi- phenotype (Hancock ; Salas-Santiago and Lopes 2014), we anticipated that NuA4 mutants would suppress the growth defect in under inositol-depleted conditions. To test this hypothesis, NuA4 mutants Δ and Δ, and the temperature sensitive mutant, (Clarke ), were crossed with and growth was assessed under both inositol-supplemented and -depleted conditions (Figure 2). As expected, Δ cells display synthetic sickness upon increased temperature in inositol-supplemented media (Curwin ), and similar interactions were seen for the double mutants of with Δ and . As was also expected, cells exhibited a growth defect in inositol-depleted media at the semipermissive temperature of 33.5° (Patton-Vogt ) (Figure 2A). While the Δ and Δ single mutants grew similarly between both conditions (Figure 2, A and B), we were surprised to see that cells displayed growth defects in inositol-depleted media even at 30° (Figure 2C). In combination, the double mutants Δ, Δ, and all showed a synthetic growth defect at 30° in inositol-depleted media compared to (Figure 2). These results suggest that, although Δ and Δ do not display detectable growth defects under inositol-depleted conditions like , these mutants do in fact exacerbate the inositol-depleted growth defects for under normally permissive temperatures. As NuA4 mutants derepress transcription and secrete excessive amounts of inositol (Hancock ; Salas-Santiago and Lopes 2014), the root cause of the growth defect under inositol-depleted conditions of Δ, Δ, and ts cells appears independent of inositol production.

Figure 2

NuA4 mutants exacerbate the growth defects of sec14-1 on inositol-depleted media. NuA4 mutants (A) eaf1Δ, (B) eaf7Δ, and (C) esa1-L254P increase the growth defects of the SEC14 temperature-sensitive mutant, sec14-1, under inositol-depleted conditions. Wild-type (YKB1079), sec14-1 (YKB3144), eaf1Δ (YKB3333), sec14-1Δ (YKB3935), eaf7∆ (YKB3292), sec14-1 (YKB4068), esa1-L254P (YKB4236), and sec14-1 (YKB4242) cultures were grown to midlog phase in SC-inositol (+75 µM myo-inositol) prior to being diluted to an OD600 of 0.1, and four times 10-fold serial dilutions were spotted on inositol-supplemented (75 µM myo-inositol) SC media or inositol-depleted SC media. Plates were incubated for 2 d at 30, 32, or 33.5° and images are representative of three biological replicates.

ICRE-regulated phospholipid genes are not fully derepressed in an EAF1 mutant background

We next sought to determine if ICRE-regulated or phospholipid genes were derepressed in a NuA4 mutant under conditions where Sec14 is inactivated, and if so, would dysregulation of these genes explain the genetic interactions between and NuA4 mutants. Using next-generation RNA-seq, we compared mRNA gene expression between and Δ. RNA samples from three biological replicates were extracted from midlog phase cells that were shifted to semipermissive temperatures (33.5°) for 2 hr to briefly inactivate . In summary, >8 million reads were obtained for each sample, identifying at least 89% of the annotated open reading frames in the Saccharomyces genome database (Cherry ; Engel ). Analysis of the ERCC spike-in standard revealed that all samples had an R2 correlation ranging from 0.92 to 0.95 (Figure S1A in File S2). These results indicate our rRNA depletion and library construction was consistent and unbiased across samples. Principal component analysis determined that the majority of the variance between samples is attributable to the differences between the two different strains and not their biological replicates (Figure S1B in File S2). Only a subset of genes was found to be significantly downregulated (103 genes, 1.84%) or upregulated (183 genes, 3.11%) in Δ compared to by a fold change of two or more and FDR adjusted p-value ≤ 0.05 (Figure 3A and File S1).

Figure 3

Transcriptional profiling of sec14-1Δ reveals that most ICRE-regulated phospholipid genes are not significantly derepressed. (A) Volcano plot for differentially expressed genes, sec14-1Δ (YKB3935) vs. sec14-1 (YKB3144), from RNA sequencing experiments. Differential expression levels of aligned sequences were calculated using significant thresholds set at log2 fold change over two and FDR adjusted p-value ≤ 0.05. Significant differentially expressed genes are in red. Blue shows the significantly changed lipid metabolic genes described in (B). (B) Table listing significantly downregulated and upregulated lipid metabolic genes. (C) Relative expression levels of ICRE-containing phospholipid genes between sec14-1Δ and sec14-1. Genes are ordered from lowest to highest fold-change expression. Genes in red are discussed further in the text.

Deletion of in the background resulted in the decreased expression of the purine biosynthesis genes (, , ) phosphate metabolic genes (, , , ) and a large cluster of genes associated with ribosomal biogenesis (File S1), which is in agreement with previously published transcriptome studies on NuA4 mutants (Reid ; Krogan ; Nourani ; Lindstrom ; Cheng ). Upregulated genes common to previous Δ transcriptome studies and our Δ transcriptome included the stress response genes (, , ) (Lindstrom ; Cheng ). Together, these results indicate that deletion of in the background impacts the transcriptome similar to what has been previously reported for NuA4 mutants in the wild-type background. However, our main purpose was to assess if ICRE-containing genes or genes implicated in phospholipid metabolism were differentially regulated by NuA4 in the background.

If NuA4 is regulating transcription of ICRE-containing genes, one would anticipate that other ICRE-containing phospholipid metabolic genes would be similarly derepressed as (Figure 3C); however, this was not the case. While the expression of the fatty acid synthases and (Kuziora ) were significantly upregulated in Δ cells, the expression of phosphatidate cytidylyltransferase (CDP-diglyceride synthetase) (Shen ; Shen and Dowhan 1997) was downregulated (Figure 3C). Indeed, the expression of the majority of ICRE-containing phospholipid genes did not display significant changes in gene expression in our transcriptome profile, including the transcription factor , whose expression remained close to basal level (Figure 3C). Derepression of expression is normally preceded by increased levels of which dimerizes with and binds to ICRE gene promoters to promote transcription (Ambroziak and Henry 1994; Ashburner and Lopes 1995). Our transcriptome analysis provides evidence of derepression occurring independently of derepression, suggesting that the transcriptional derepression of in Δ is not characteristic of the typical Opi- transcriptional response.

Extending our search beyond just ICRE-regulated genes, we were surprised to find that only eight genes involved in phospholipid metabolism displayed significant transcriptional change between and Δ (Figure 3B). In addition to , downregulated genes included the SE hydrolase (Koffel ), the phospholipase B (Fyrst ), and , which encodes a protein implicated in phosphatidylinositol-4,5-bisphosphate synthesis (Audhya and Emr 2003). Upregulated genes included the inositol-3-phosphate synthase , the phospholipase B (Merkel ), and and . As recent evidence suggests that the contribution of phospholipase B enzymes toward phospholipid turnover in vivo is negligible (Mora ), we focused our attention on the remaining six genes. For each of the lipid metabolic genes, the changes in expression detected by next-generation sequencing analysis were confirmed through qRT-PCR (Figure S2 in File S2).

The misregulation of a handful of phospholipid metabolic genes, most notably that of , suggests that perturbation of phospholipid homeostasis may contribute to the growth defects displayed in Δ under inositol-depleted conditions. Given the essential role of , we predicted that its downregulation in Δ may be contributing to this negative genetic interaction. However, we were surprised to discover that the overexpression of in Δ could not rescue the growth defects under inositol-depleted conditions (Figure S3 in File S2). Therefore, downregulation of by itself is not the cause of the growth defects in Δ.

Lipid droplet dynamics is impaired in eaf1Δ cells

We next wanted to determine which, if any, lipid metabolic pathways were affected in Δ cells that might explain the genetic interaction between and Δ. We opted to explore if the growth defect in Δ under inositol-depleted conditions is potentially due to defects in TAG and SE biosynthesis for two reasons. First, we found altered expression of , , and , which all encode proteins implicated in neutral lipid synthesis (reviewed in Eisenberg and Buttner 2014; Fernandez-Murray and McMaster 2016) (Figure 1). Second, under inositol-depleted conditions, cells require inositol as well as the ability to synthesize both TAG and SE (both neutral lipids) for survival (Gaspar ). TAG and SE biosynthesis can be completely abolished in yeast by deleting , , , and , genes encoding the proteins responsible for all neutral lipid biosynthesis in yeast (Oelkers ; Sandager ). Intriguingly, like Δ strains, a yeast strain in which all TAG and SE biosynthesis is abolished (ΔΔΔΔ) is not able to grow in the absence of inositol at higher temperatures despite expression (Gaspar ). The formation of lipid droplets is an established proxy for TAG and SE biosynthesis (Wang 2015); therefore, we examined lipid droplet formation under inositol-supplemented and -depleted conditions in the wild-type, , Δ, and Δ strains at 30° using a fluorescent lipid droplet marker. As expected, upon inositol depletion, wild-type cells display a nearly threefold increase in fluorescence of the lipid droplet marker, whereas there is no increase in ΔΔΔΔ cells where TAG and SE biosynthesis is abolished (Figure 4 and Figure S4 in File S2) (Gaspar ). Much like wild-type cells, upon inositol depletion, cells emitted a nearly threefold increase in fluorescence density compared to inositol-supplemented conditions (Figure 4, A and B). In contrast, deletion of in either the wild-type or background resulted in a reduction in the fluorescence intensity of lipid droplets, which suggests that some aspect of lipid droplet dynamics is significantly impaired in Δ cells. Furthermore, although the reduction of fluorescence intensity of lipid droplets was not as striking in Δ and Δ cells, it was clearly reduced in -L254P and cells. As both Δ and -L254P cells display reduced KAT activity, this suggests that the catalytic activity of the NuA4 complex is involved in the regulation of lipid droplet and potentially neutral lipid biosynthesis (Figure S5 in File S2). If the defect in lipid droplets seen in NuA4 mutant cells is a reflection of neutral lipid biogenesis, this potentially could explain the increased growth defects of Δ, Δ, and cells under inositol-depleted conditions.

Figure 4

Lipid droplet dynamics is impaired in EAF1 deletion mutants. (A) Wild-type (YKB1079), sec14-1 (YKB3144), eaf1Δ (YKB3333), and sec14-1Δ (YKB3935) cultures were grown to midlog phase in SC media at 30° before shifting to inositol-supplemented (75 µM myo-inositol) SC media or inositol-depleted SC media for 2 hr at 30° prior to being stained with 10 µM BODIPY 493/503 for 10 min before imaging. Images shown are midfield view of representative cells for each sample (scale bar, 10 µm). (B) Graphic display of the mean relative fluorescence density for each strain and condition. Cells were first segmented from brightfield images using a custom MATLAB script then fluorescence was measured for each cell using the outlines (see Materials and Methods for details). Mean fluorescence density was measured from 100 cells across three biological replicates relative to wild-type fluorescence in inositol-supplemented media (+SEM). Statistical analysis was performed by one-way ANOVA with Tukey’s multiple comparisons test: **p < 0.05; n.s., not significant.

Inhibition of de novo fatty acid biosynthesis has a detrimental effect on sec14-1ts growth

To investigate if the genetic interaction between and Δ was due to a role of Eaf1 (and presumably NuA4) in neutral lipid biosynthesis, we examined the growth of strains when both TAG and SE biosynthesis are eliminated (Figure 5A). As previously shown, ΔΔΔΔ (d.l.a.a.Δ in Figure 5) cells do not display defects on inositol-supplemented media, but become inositol auxotrophs at 37° (Gaspar ) (Figure 5A). If the genetic interaction between ts and Δ was due to decreased neutral lipid biosynthesis caused by deletion of , we would predict that ΔΔΔΔ cells would display similar growth defects on inositol-depleted media as Δ. However, in inositol-supplemented or -depleted conditions at 30°, ΔΔΔΔ combined with does not impair growth. Further, the addition of ΔΔΔΔ does not increase the growth defects of Δ cells at 30°. Indeed, we detect a negative genetic interaction between Δ and ΔΔΔΔ on inositol-supplemented media at 37°, suggesting that Eaf1, and presumably NuA4, function in separate pathways. Altogether, this suggests the growth defect in Δ under inositol-depleted conditions or at higher temperatures is not the result of Δ mutant defects in neutral lipid biosynthesis.

Figure 5

Inhibition of fatty acid biosynthesis causes a synthetic growth defect in sec14-1ts. (A) Genetic inhibition of triacylglycerol and steryl ester biosynthesis does not affect the growth of sec14-1. Wild-type (YKB1079), dga1Δlro1Δare1Δare2Δ (d.l.a.a.Δ; YKB4336), sec14-1 (YKB3144), sec14-1.Δ (YKB4337), eaf1Δ (YKB3333), eaf1Δd.l.a.a.Δ (YKB4338), sec14-1Δ (YKB3935), and sec14-1Δ d.l.a.a.Δ (YKB4339) cultures were grown in YPD at 30° prior to being diluted to an OD600 of 0.1, and four times 10-fold serial dilutions were plated on inositol-supplemented (75 µM myo-inositol) SC media or inositol-depleted SC media and incubated for 2 d at 30°. (B) Inhibition of fatty acid biosynthesis by cerulenin treatment causes synthetic growth defect with sec14-1. Wild-type (YKB1079), sec14-1 (YKB3144), eaf1Δ (YKB3333), and sec14-1Δ (YKB3935) cultures were grown in YPD at 30° prior to being diluted to an OD600 of 0.1, and four times 10-fold serial dilutions were plated on YPD with indicated amounts of cerulenin for 2 d at 30, 32, 33.5, and 37°. Images are representative of three biological replicates.

Though a reduction in neutral lipid biosynthesis does not explain the inositol-depleted growth defects of Δ cells, the reduction of lipid droplet staining in NuA4 mutant cells suggests a potential defect(s) within this pathway (Figure 4 and Figure S5 in File S2). Therefore, we examined whether the de novo biosynthesis of fatty acids (Figure 1), a requisite precursor for neutral lipid biosynthesis, was involved in the negative genetic interaction between and Δ. For this purpose, we used cerulenin, a fatty acid analog that inhibits the enzymatic activity of fatty acid synthases and (Kawaguchi , 1982), to determine the effect of inhibiting fatty acid biosynthesis on growth. We found that while the growth of wild-type and Δ cells were not impacted by 2.5 µM cerulenin treatment at 30°, growth of cells were hypersensitive to cerulenin treatment, suggesting that fatty acid biosynthesis is especially critical for the survival of this strain (Figure 5B). Interestingly, the cerulenin sensitivity of cells at 30° was rescued by deletion of . However, at 32° and 33.5°, cerulenin treatment affected ts growth to a similar extent as Δ in the absence of cerulenin treatment, and the deletion of in the s background did not increase sensitivity to cerulenin treatment at 32°. Moreover, at 37°, Δ cells normally display a growth defect compared to wild-type cells; however, upon cerulenin treatment, wild-type cells lose their growth advantage, with both wild-type and Δ cells displaying comparable growth. A similar buffering effect was also seen with Δ and mutants upon cerulenin treatment (Figure S6 in File S2). This suggests a role for NuA4 within the fatty acid biosynthesis pathway that helps buffer the inhibition of the fatty acid synthases. Taken together, this work suggests that the Δ mutant negative genetic interaction with ts and the decreased lipid droplet staining in Δ originate from defects within the fatty acid biosynthesis pathway.

Discussion

Here we set out to begin to dissect the biological role for NuA4 in phospholipid homeostasis. Surprisingly, we found that NuA4’s role in inositol auxotrophy is not simply a reflection of regulation of ICRE-regulated phospholipid genes. Rather, through dissection of the genetic interaction between and Δ, our work provides evidence for a role of NuA4 in contributing to the regulation of neutral lipid and fatty acid biosynthesis pathway.

NuA4 mutants increase the inositol auxotrophy of sec14-1ts cells despite INO1 derepression

NuA4 mutants are known to exhibit the Opi- phenotype, which is the overproduction of inositol caused by the derepression and transcription of (Hancock ; Salas-Santiago and Lopes 2014). As deletion mutants of the CDP-choline pathway that exhibit an Opi- phenotype suppress the growth defect in the mutant under inositol-depleted conditions (Patton-Vogt ; Chang ), we initially hypothesized that the introduction of NuA4 mutants into a background would rescue growth on inositol-depleted media. Instead, we found that the combination of and NuA4 mutants resulted in an increased growth defect under inositol-depleted conditions despite derepression (Figure 2, Figure 3, and Figure S2A in File S2). However, comparative to Δ cells that are considered to have a strong Opi- phenotype, NuA4 mutants display only an intermediate Opi- phenotype, as determined by the extent of the depression of an reporter gene (Hancock ). Similarly, our transcriptome analysis indicated only a twofold derepression of expression (Figure 3), which differs considerably from the 56.7-fold increase in an Δ background (Santiago and Mamoun 2003). Despite this fact, we did not expect the growth defect in under inositol-depleted conditions to worsen in combination with NuA4 mutants. This suggests that survival under inositol-depleted conditions requires more than just induction and inositol production. Our transcriptional data showed that partial derepression and transcription of was occurring in Δ, but derepression was not extended to all ICRE-regulated phospholipid genes. The main transcriptional activator of ICRE-regulated genes, , which is normally induced under similar conditions as , remained at basal levels of transcription in Δ cells (Figure 3). This suggests that the induction of in Δ cells and other NuA4 mutants (Hancock ; Salas-Santiago and Lopes 2014) may not be dependent on , potentially explaining why most ICRE-regulated genes are not induced in Δ cells.

One possible mechanism for the induction of expression in Δ cells could be through the downregulation of expression (Figure 3 and Figure S2D in File S2). It has been shown that lowering expression of the essential gene causes an Opi- phenotype and induction of expression independent of derepression, much like NuA4 mutants (Shen and Dowhan 1996, 1997; Salas-Santiago and Lopes 2014). Therefore, it is possible that the Opi- phenotype previously reported for NuA4 mutants is caused by the downregulation of expression. However, reduction of causes an increase in both PA and TAG levels, resulting in supersized lipid droplets (Fei ), which is not seen in Δ cells (Figure 4). Furthermore, we have shown that overexpressing does not rescue the growth phenotype of our Δ strain (Figure S3 in File S2). One intriguing possibility is the Opi- phenotype of NuA4 mutants is an indirect consequence of the cell trying to compensate for defects in TAG and SE biosynthesis, resulting in the reduction of . Indeed, it remains to be determined if NuA4-dependent acetylation of histones is directly regulating the transcription of the eight lipid metabolism genes identified in our screen, or if the changes in gene expression reflect a transcriptional compensation mechanism independent of NuA4’s nuclear activity.

Is NuA4 regulating lipid droplet dynamics through the fatty acid biosynthesis pathway?

A decrease in lipid droplet staining despite the derepression of expression is also a characteristic of the quadruple mutant ΔΔΔΔ, which is unable to synthesize neutral lipids (Figure S4 in File S2) (Mullner and Daum 2004; Gaspar ). Further, like our mutant cells (Figure 2C), ΔΔΔΔ cells are sensitive to inositol-depleted conditions at higher temperatures (Figure 5A) (Gaspar ). However, the loss of neutral lipid biosynthesis did not account for the negative genetic interaction between NuA4 and Sec14 mutants, nor did it account for the increased growth of Δ on inositol-depleted media at 30° (Figure 5A).

An alternative explanation could be that defective lipid droplet formation in Δ and other NuA4 mutants is caused by a lack of fatty acid substrate. We demonstrated that the inhibition of the fatty acid biosynthesis pathway by cerulenin dramatically increased the growth defect in (Figure 5B and Figure S6 in File S2). As the deleterious effect of cerulenin treatment on is only mildly additive to the growth defects incurred by NuA4 mutants at 32°, it would suggest that fatty acid biosynthesis may already be compromised in NuA4 mutants at higher temperatures. Indeed, this could account for the limited impact of cerulenin treatment on Δ cells compared to wild-type cells at 37°. The suppressive effect of Δ, Δ, and on cerulenin treatment compared to at 30° remains unresolved. Potentially, increased expression of both and in Δ (Figure 3 and Figure S2, B and C in File S2), and presumably other NuA4 mutants, may be able to buffer the effects of cerulenin at 30°; however, at higher temperatures, increased expression may not be able to buffer the defects within this pathway manifested by deletion of . The fact remains that the effect of inhibiting fatty acid synthases in cells is largely nonadditive to the effect of NuA4 mutants, which suggests an epistatic interaction between NuA4 and .

Our proposed theory that NuA4 positively regulates the fatty acid biosynthesis pathway accounts for most of the phenotypes reported in this paper. Inhibition of the fatty acid biosynthesis pathway negatively affects neutral lipid biosynthesis and lipid droplet formation as they are the principal substrates in these pathways (Henry ; Wang 2015). Similar to NuA4 mutants, downregulation of the fatty acid biosynthesis pathway leads to the derepression and transcription of (Shirra ). Whether the inhibition of the fatty acid biosynthesis pathway is the primary cause behind transcriptional activation in NuA4 mutants remains to be confirmed. Conversely, the opposite effect is observed when this pathway is activated. Overexpression of genes responsible for fatty acid biosynthesis represses the transcription of (Shirra ; Feddersen ) and increases fatty acid biosynthesis, causing a dramatic accumulation of lipid droplets (Hofbauer ).

How is NuA4 regulating the fatty acid biosynthesis pathway? Our work suggests that NuA4 is a positive regulator of the fatty acid biosynthesis pathway. Based on this theory, one potential mechanism is through NuA4-dependent transcriptional regulation of fatty acid biosynthesis genes. However, transcriptome analysis on NuA4 mutant subunits have not identified significant decreases in fatty acid biosynthesis genes (Krogan ; Lindstrom ; Cheng ). Indeed, our work identified an increase in mRNA expression of and in Δ cells, which may reflect the cells’ attempts at compensating for decreased lipogenesis flux upon deletion of (Figure 3). NuA4 has also been implicated in the inhibition of AMPK1/Snf1, and NuA4 mutants display hyperactivated Snf1 (Lu ). As Snf1 phosphorylates and inhibits the activity of acetyl-CoA carboxylase (Acc1), the first step of fatty acid de novo synthesis (Hofbauer ), NuA4 maybe regulating fatty acid biosynthesis pathway by reducing Snf1 activity and maintaining Acc1 activity. Indeed, activity of Acc1 is reduced in WCEs from NuA4 mutants (Rollins ). Alternatively, and perhaps not mutually exclusively, NuA4 may also have potential targets within the fatty acid biosynthesis pathway. In fact, lysine acetylation of proteins in this pathway, including Fas1 and Fas2, have been detected in both yeast and higher organisms (Choudhary ; Henriksen ; Weinert ; Downey ; Madsen ). While the mechanism(s) through which NuA4 is contributing to cellular lipid homeostasis remain unclear, our work shows that NuA4 has underappreciated roles in lipid homeostasis.

Supplementary Material

Supplemental material is available online at www.g3journal.org/lookup/suppl/doi:10.1534/g3.117.041053/-/DC1.

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