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NuA4 histone acetyltransferase activity is required for H4 acetylation on a dosage-compensated monosomic chromosome that confers resistance to fungal toxins
Epigenetics & Chromatin volume 10, Article number: 49 (2017)
The Correction to this article has been published in Epigenetics & Chromatin 2017 10:52
The major human fungal pathogen Candida albicans possesses a diploid genome, but responds to growth in challenging environments by employing chromosome aneuploidy as an adaptation mechanism. For example, we have shown that C. albicans adapts to growth on the toxic sugar l-sorbose by transitioning to a state in which one chromosome (chromosome 5, Ch5) becomes monosomic. Moreover, analysis showed that while expression of many genes on the monosomic Ch5 is altered in accordance with the chromosome ploidy, expression of a large fraction of genes is increased to the normal diploid level, presumably compensating for gene dose.
In order to understand the mechanism of the apparent dosage compensation, we now report genome-wide ChIP-microarray assays for a sorbose-resistant strain harboring a monosomic Ch5. These data show a significant chromosome-wide elevation in histone H4 acetylation on the mCh5, but not on any other chromosome. Importantly, strains lacking subunits of the NuA4 H4 histone acetyltransferase complex, orthologous to a complex previously shown in Drosophila to be associated with a similar gene dosage compensation mechanism, did not show an increase in H4 acetylation. Moreover, loss of NuA4 subunits severely compromised the adaptation to growth on sorbose.
Our results are consistent with a model wherein chromosome-wide elevation of H4 acetylation mediated by the NuA4 complex plays a role in increasing gene expression in compensation for gene dose and adaption to growth in a toxic environment.
Candida albicans is an opportunistic fungal pathogen that is part of the normal microbial community of the digestive tract and genitalia of humans. C. albicans does no harm to the healthy host; however, it causes life-threatening infections in severely immunocompromised patients. C. albicans normally possesses a diploid genome organized in eight pairs of chromosomes, but uses reversible loss or gain of an entire chromosome or a large part of chromosomes to survive in toxic environments that would otherwise kill cells or prevent their propagation [reviewed in 1, 2]. For example, the loss of one chromosome 5 (Ch5) or duplication of the right arm of Ch5 confers laboratory resistance to the anti-fungal caspofungin [3, 4]. The loss of one Ch5 also confers laboratory resistance to the anti-fungal flucytosine, as well as resistance to toxic sugar l-sorbose, which kills C. albicans in a manner similar to caspofungin or other frontline drugs from the echinocandin class [reviewed in 3]. In addition, changes in Ch5 ploidy are frequently found in fluconazole-resistant clinical isolates of C. albicans [reviewed in 5, 6]. In light of data pointing to the importance of Ch5 in C. albicans drug resistance, there is a growing need to better understand the control of Ch5 ploidy and regulation of genes on this chromosome.
Previous studies of changes in transcription of Ch5 genes associated with the loss of one Ch5 in a mutant [Sor125(55)] adapted to growth on the toxic sugar sorbose (Sou+) revealed expression of many genes on the monosomic Ch5 decreased twofold, conforming to the loss of DNA copy number. However, surprisingly, expression of ~ 40% of gene transcripts from monosomic Ch5 corresponded to the normal disomic or near disomic levels . In addition to monosomy of Ch5, this mutant acquired duplication of a chimeric Ch4/7b, resulting in trisomy of this chromosome (Fig. 1a), and facilitating the Sou+ phenotype . Similar to Ch5, our data show that while expression of many genes on the trisomic Ch4/7b increased 1.5-fold, as expected from gene copy number, many other genes were expressed at the normal disomic or near disomic levels (C. Tucker and E. Rustchenko, unpublished observation). These observations led us to propose that in C. albicans, transcriptional compensation for gene dose serves to facilitate the formation and maintenance of aneuploid chromosome states that are required for survival in adverse environments . We have previously reported multiple genes encoding negative regulators of laboratory resistance to echinocandins or sorbose that are scattered across Ch5 . While the final number of regulatory genes is yet to be determined, some are involved in cell wall biosynthesis, while others important to the Sou+ and drug susceptibility phenotypes are subjects of antisense regulation [9,10,11]. However, despite these advancements, little is known about the formation and maintenance of the monosomic Ch5 state.
The regulation of gene expression on the monosomic Ch5 in C. albicans is possibly analogous to the well-described and essential dosage compensation found on the single male X chromosome in Drosophila melanogaster. In this organism, compensation requires histone H4 acetylation mediated by the male-specific lethal (MSL) complex, which includes the histone acetyltransferase (HAT) subunit MOF . MSL acetylation of H4 is associated with twofold upregulation of almost all genes on the single X chromosome. The orthologous complex in C. albicans is termed the nucleosome acetyltransferase of H4 (NuA4) complex, in which the Esa1p subunit harbors the catalytic activity . The NuA4 complex is evolutionarily conserved from yeast to humans and is known to be a key regulator of transcription [14, 15]. In Saccharomyces cerevisiae, NuA4 is responsible for the acetylation of nucleosomal histone H4 at lysine K5, K8, and K12 and, to a lesser extent, at K16. In C. albicans, NuA4 contributes mainly to acetylation of H4 K5 and H4 K12, whereas the SAS HAT complex contributes to acetylation of H4 K16 . In support, deletion of a gene encoding the NuA4 catalytic subunit Esa1p in C. albicans significantly diminished acetylation of H4 K5 and H4 K12 . Also, deleting Nbn1p, which comprises part of the NuA4 catalytic module, diminished overall H4 acetylation .
Considering the well-characterized model of dosage compensation mechanisms operative on the single X chromosome of D. melanogaster, we wished to determine whether elevated H4 acetylation is similarly associated with the aforementioned widespread transcriptional upregulation found on the monosomic Ch5 in the C. albicans sorbose-resistant mutant . Indeed, we found increased H4 acetylation exists across the monosomic Ch5, while, in contrast, increased H3 acetylation is found within the trisomic Ch4/7b region. Importantly, we show that NuA4 subunits are required for elevated H4 acetylation in strains bearing a monosomic Ch5 and for efficient adaption to growth of C. albicans in the presence of the toxic sorbose.
Acetylation of H4 and H3 on aneuploid chromosomes in C. albicans
We first asked whether histone H4 acetylation patterns across the genome are altered in the well-characterized sorbose-resistant strain Sor125(55) containing a monosomic Ch5 and a trisomic Ch4/7b, compared to the normal diploid parental strain (Fig. 1a). We performed chromatin immunoprecipitation on chip (ChIP-Chip) using a pan-H4-acetylation antibody with hybridization to our custom tiling arrays (see “Methods”). Analysis of the data shows sporadic changes in acetylation genome wide, with both increases and decreases apparent at many loci (Fig. 1b, note that the majority of loci have changes that do not exceed a threshold and are not plotted). However, we observed a generalized and much larger fivefold to tenfold increase in H4 acetylation on the monosomic Ch5 than that found on all other chromosomes. All chromosomes showed similar amounts of decreased H4 acetylation.
We then asked whether the greatly elevated level of histone acetylation we observe on the monosomic Ch5 is specific to histone H4 or a more generalized feature of nucleosomes in the mutant strain by examining genome-wide acetylation of histone H3, which is also commonly increased in association with transcription. We performed ChIP-Chip using an antibody specific for H3 acetylated at the transcription-related sites K9 and K14 and found that H3 acetylation on Ch5 appeared similar to that found on all other disomic chromosomes, exhibiting a sporadic pattern of increases and decreases at various loci in the mutant compared to the parental strain. In contrast, we detected approximately a twofold to tenfold overall increase in H3 acetylation localized to the trisomic Ch4/7b region of the genome (Fig. 1b).
We also noticed a number of large negative peaks in the H4 acetylation plot, indicating loci exhibiting significant decreases in this modification in the mutant compared to parental cells (marked with asterisks in Fig. 1b, note that many of these peaks are too closely positioned to be distinguished in this figure, but are listed in Additional file 1: Table S1). There were 43 such peaks scattered throughout the genome, associated with 27 open reading frames (ORFs) based on the criteria of being positioned either within 1 kb of an ORF or within of an ORF. The function of the majority of the peak-associated genes is not known, thus understanding the phenotypic outcome associated with these changes in acetylation awaits further analysis.
The NuA4 complex plays a role in elevated H4 acetylation on the monosomic Ch5
As described above, elevated histone acetylation associated with dosage compensation of the single X chromosome in male flies is due to the HAT MOF that acetylates histone H4 . To determine whether the orthologous NuA4 complex in C. albicans is involved in the large increase in acetylation observed across Ch5 in sorbose-resistant [Sor125(55)] cells, we initially employed three C. albicans strains, each with the NuA4 complex disrupted. Specifically, we employed strain Nbn1 (nbn1 −/−) in which both alleles of the NBN1 (orf19.878) gene encoding the Nbn1p subunit of the catalytic NuA4 HAT module are deleted. We also used the strain Eaf3 (eaf3 −/−), in which both alleles of orf19.2660, encoding Eaf3p, an ortholog of yeast EAF3 within the targeting module of the S. cerevisiae NuA4 complex, are deleted. Finally, we employed strain Esa1 (esa1 −/+), in which one allele of the essential ESA1 (orf19.5416) gene encoding the catalytic subunit of the NuA4 complex is disrupted (Table 1). PCR and Southern blot analyses confirmed disruption of one ESA1 allele and deletion of both alleles of NBN1 and EAF3 in these strains (data not shown).
We first tested how loss of the NuA4 subunits affected the growth of Esa1, Nbn1 or Eaf3 cells, as compared to their parent strains. We spread approximately 3000 colony-forming units (cfu) of each strain on plates with YPD universal rich medium and, when micro-colonies appeared, measured number of cells in colonies in approximately 4-h intervals. We found that the loss of Nbn1p from the catalytic module of the NuA4 complex greatly affected the growth, whereas the loss of Eaf3p from the targeting module or disruption of one copy of ESA1 encoding the NuA4 catalytic subunit had little effect on growth (Fig. 2). The Esa1 strain was not included in further experiments because the effect of disruption of a single copy of ESA1 might not result in NuA4 insufficiency [for example, see 9].
We next assessed whether disruptions of the NuA4 complex altered histone acetylation levels upon transition of Nbn1 or Eaf3 cells from disomic to monosomic state of Ch5. We generated monosomic Ch5 mutants from the NuA4+ parental strain DAY286 and the NuA4 deletion mutants Nbn1 and Eaf3 (Table 1) using our well-established method of plating cells on l-sorbose medium  (see “Methods”). We confirmed loss of one Ch5 in derived mutants by PCR with primers for MTL loci, residing on Ch5 . We also examined the chromosome banding pattern in one mutant from each parental strain by pulse-field gel electrophoresis (PFGE) (Additional file 2: Figure S1). PFGE analysis showed that ChR carrying tandem repeats of ribosomal DNA (rDNA) units exhibited some instability in the Nbn1 monosomic Ch5 mutant as expected, since changes of ChR lengths frequently occur due to changes in the number of rDNA units in the cluster of tandemly assembled rDNA units . Otherwise, chromosome banding patterns did not show any other alterations in mutant strains other than monosomy of Ch5, common to all mutants. It is important to note that adaptation of C. albicans to growth on sorbose as the sole source of carbon almost exclusively involves a transition to a monosomic Ch5 state without other chromosome alterations, in multiple genetic backgrounds (> 95% incidence) [3, reviewed in 1, 2, 20], and this method is now used by many laboratories.
Having established the monosomic Ch5 strains in the desired parental and deletion backgrounds, we next employed Western blot analysis with either pan-acetyl H4 antibody or antibodies, specific for acetylation at H4 K5, H4 K12, or H4 K16 to compare acetylation in these strains. Importantly, we found a significant increase in total acetylation of H4 in the Sor125(55) strain that harbors a monosomic Ch5, compared to the parent 3153A (Fig. 3a, also see Additional file 3: Figure S2), consistent with our ChIP analysis (Fig. 1b). Likewise, we observed a significant total increase in H4 acetylation in the newly generated monosomic Ch5 mutant DAY286-1 versus its parent DAY286 (Fig. 3a, also see Additional file 3: Figure S2). Increased acetylation was also detectable with antibodies specific for H4 K5ac or K12ac [Sor125(55)], or H4 K5ac (DAY286-1). These data are in good agreement with our genome-wide ChIP analyses and indicate that the large elevation of H4 acetylation specific to Ch5 in strains monosomic for Ch5 can be observed in blots of histones isolated from whole cells.
We next compared H4 acetylation in parental cells lacking subunits from the NuA4 HAT and strains harboring a monosomic Ch5 derived from these cells. In a strain lacking the Nbn1 subunit from the catalytic module of NuA4, we found no difference in overall H4 acetylation compared to the parental DAY286 (Fig. 3b, black bar) and no significant difference was detected with antibodies specific for single acetylation events in the H4 tail (Fig. 3b, gray, hatched and white bars). Importantly, in contrast to Ch5 monosomic strains with a fully functional NuA4 complex, we found no increase in H4 acetylation associated with transition of the Nbn1 deletion strain to a monosomic Ch5 state (Fig. 3a, Nbn1-1, black bars). See results for two more independent Ch5 monosomic derivatives of Nbn1 in Additional file 4: Figure S3. The result was similar whether comparing pan-acetylation of H4 or specific acetylation at individual H4 lysines (Fig. 3a, Nbn1-1, gray, hatched, and white bars). Likewise, in cells lacking the Eaf3p subunit from the targeting module of NuA4, no increase in overall acetylation was observed upon transition from a disomic to monosomic Ch5 state (Fig. 3a, compare Eaf3 and Eaf3-1). Our results indicate that the elevated H4 acetylation observed in mutants with monosomic Ch5 is due to the activity of the NuA4 complex.
Role of the NuA4 complex in formation of the monosomic Ch5
To determine whether the NuA4 complex has a role in formation of the monosomic Ch5 state, we determined whether the rates of production of Sou+ cells monosomic for Ch5 are affected by deletion of Nbn1 or Eaf3 subunits compared to the parental strain DAY286. The experiments were conducted, as previously reported . Production of Sou+ colonies representing Sou+ mutants was observed for each strain by spreading from 2 × 105 to 6 × 105 of the Sou− cells on l-sorbose plates in three independent experiments. The appearance of Sou+ colonies was recorded daily and is presented as an averaged accumulation curve (Fig. 4a). Survival of Sou− cells was assessed from sorbose plates by daily transfer of entire agar disks to YPD plates, incubation for 3 days, and counting the number of grown colonies [see 18 for more details]. The daily survival of Sou− cells of each strain is presented in Additional file 5: Figure S4. The daily rate of production of Sou+ mutants was calculated by dividing the number of Sou+ colonies appearing daily by number of cells that were viable 4 days earlier, the predicted day of the mutational events leading to transformation (Fig. 4b). [For example, we considered that mutational events that occurred in parental DAY286 cells on day 0 would result in appearance of visible Sou+ colonies on day 4 (Fig. 4a)]. We found greatly diminished rates of Sou+ mutants’ production with strains Nbn1 and Eaf3 lacking NuA4 subunits versus DAY286 with a normal NuA4 complex. This result shows that efficient adaptation to sorbose by formation of the monosomic Ch5 depends on the NuA4 complex.
In this work, we show that a chromosome-wide increase in acetylation of histone H4 occurs on the single Ch5 of the C. albicans sorbose-resistant mutant Sor125(55), on which ~ 40% of genes are upregulated to disomic or near disomic levels, thus compensating for decreased gene dosage. Such an increase in H4 acetylation seems to be a general attribute of the monosomic Ch5 state, as it also occurred on the single Ch5 in the mutant DAY286-1, which has a different genetic background. Increased H4 acetylation, however, does not occur on the trisomic Ch4/7b in the Sor125(55) mutant, on which multiple genes are downregulated to disomic or near disomic levels, again compensating for increased gene dosage (E. Rustchenko, unpublished observation). Instead, a chromosome-wide increase in acetylation of histone H3 occurs on the trisomic Ch4/7b, but does not occur on the monosomic Ch5 or any disomic chromosome. Thus, unique epigenetic signals occur on chromosomes with different aneuploidies, consistent with distinct transcriptional responses. We provide evidence that the bulk of the increased acetylation of histone H4 is due to activity of the NuA4 HAT complex, orthologous to the enzyme complex previously implicated in dosage compensation on the single male X chromosome in Drosophila. While the enzymes responsible for the observed increase in H3 acetylation have yet to be identified, previous work in C. albicans suggests that the Rtt109 or SAGA/ADA complexes might be responsible [21, 22].
Interestingly, disruption of a single allele of the essential ESA1 gene encoding the catalytic subunit of the NuA4 complex or lack of the Eaf3p subunit from targeting module did not have a significant effect on strain viability. These results suggest that sufficient Esa1p is produced in the hemizygous Esa1 strain for cell survival and Eaf3p is not critical for survival. Also, whole-cell Western blotting showed that strains lacking NuA4 subunits Nbn1p or Eaf3p did not exhibit reduced H4 acetylation attributable to NuA4. However, Wang et al.  reported that deletion of the NuA4 catalytic subunit Esa1p resulted in a significant decrease in the acetylation level of C. albicans nucleosomal H4. Importantly, deletion of either the Nbn1p or Eaf3p subunits of the NuA4 complex eliminated the characteristic increase in H4 acetylation observed on the monosomic Ch5 in DAY286-1 and compromised the ability of the deletion strains to undergo transformation to a monosomic Ch5 state. Our results support a model wherein a major pathway to generation of sorbose-resistant C. albicans mutants involves adaptation of a monosomic Ch5 state, with a concurrent chromosome-wide increase in H4 acetylation to facilitate a twofold upregulation of the large proportion of Ch5 genes required for normal cellular homeostasis.
We find consistency in the fact that there are epigenetic changes on both aneuploid chromosomes in Sor125(55), monosomic Ch5 and accompanying trisomic Ch4/7b. Although the details of gene regulation on Ch4/7b are less understood, and will be the subject of future study, the increase in acetylation of H3 is likely to be the outcome of a mechanism distinct than that responsible for upregulating expression of single-copy genes on Ch5. This mechanism might be involved in upregulation of a subset of genes on the trisomic Ch4/7b in conjunction with the increase in gene dosage associated with sorbose adaptation, concomitant with compensatory downregulation of many other genes to the disomic level. Given that mutants were preserved immediately after generation, we believe that the increase in H3 and H4 acetylation we detected is directly coupled with generation of aneuploid states and not with an unspecified instability due to, for example, how cells were maintained and handled (see “Methods”).
Our results suggest NuA4 as a novel drug target to reduce the viability of strains resistant to anti-fungals. We have shown that a significant fraction of sorbose-resistant mutants with a monosomic Ch5 also exhibit decreased susceptibility to the anti-candidal agent caspofungin . In addition, approximately a quarter of mutants that adapted to caspofungin upon direct exposure to this drug transitioned to a monosomic Ch5 state, which defines the decreased drug susceptibility . Interestingly of over 20 HATs in S. cerevisiae, only Esa1p, the catalytic subunit of NuA4, is essential for viability . In C. albicans NuA4, four subunits (Esa1p, Nbn1p, Eaf6p, and Epl1p) comprise the catalytic core, while eight, including Eaf3p, make up a structural/targeting module . Given its role in resistance, drugs that act upon the NuA4 complex in Candida, but not in humans could provide a pathway to combating C. albicans infections.
Our data imply that acetylation associated with the monosomic Ch5 requires critical subunits of the C. albicans NuA4 HAT complex, suggesting a mechanism similar to that operative on the single X chromosome in Drosophila males, and setting a precedent for a fundamental cellular process appearing earlier in evolution. Recently, transcriptional dosage compensation was reported for sets of genes on different trisomic or higher ploidy aneuploid chromosomes in wild or laboratory strains of S. cerevisiae . However, to our knowledge, no report is available regarding the state of histone acetylation on aneuploid chromosomes in S. cerevisiae. It will be interesting in future experiments to determine how NuA4 HAT activity contributes to the generation of monosomic Ch5 strains and the role of increase in H3 acetylation on Ch4/7b.
Strains, media, and growth conditions
The parental strain BWP17  and a derivative strain Esa1 in which one copy of the gene ESA1 encoding a catalytic subunit of NuA4 HAT complex is disrupted were supplied from the Tag-Module collection, University of Toronto. The parental strain DAY286 , a derivative strain Nbn1, lacking the NBN1 gene encoding a subunit from the catalytic module of the NuA4 complex, and a derivative strain Eaf3, lacking the EAF3 (orf19.2660) gene encoding a subunit identified as a component of the targeting module of yeast S. cerevisiae NuA4, were supplied by Fungal Genetics Stock Center (FGSC), University of Missouri, Kansas City (http://www.fgsc.net/candida/FGSCcandidaresources.htm). All the above strains cannot utilize sorbose, Sou−, and die on medium in which toxic sorbose is available as the only carbon source . Also, we used the Sou− strain 3153A and its Sou+ derivative Sor125(55)  (see Fig. 1a for schematics of chromosome ploidy of these strains). See Table 1 for strains used in this work.
Yeast extract/pepton/dextrose (YPD), synthetic dextrose (SD), l-sorbose, or sorbitol media were previously described [11, 28]. Media were supplemented with uridine (50 µg/ml), histidine (20 µg/ml), or arginine (10 µg/ml) when needed, as previously indicated . Strains were preserved as − 70 °C stocks immediately after generation of mutant colonies and handled such that to avoid accumulation of unspecified mutations and chromosome instability due to, for example, long-term propagation, the use of aged cultures or exposure to low temperatures [see 29, 30 for more].
Generation and analysis of Ch5 monosomic mutants
Mutants that lost one Ch5 were generated by plating cells on solid synthetic medium in which l-sorbose is substituted for glucose as described [3, 18]. Intact chromosomes were prepared and precisely separated using contour-clamped homogenous electrophoretic field (CHEF) version of PFGE, as described .
We performed chromatin immunoprecipitation (ChIP) as described previously . Briefly, cells were transferred from − 70 °C stocks to sorbitol master plates as a streak and incubated overnight, and approximately 3500 cfu were plated on each sorbitol plate to generate independent colonies. Upon reaching approximately 1 × 105 cells per colony, cells were collected and frozen at − 70 °C. Next, cells were removed from − 70 °C and proteins and DNA were formaldehyde cross-linked, cells were lysed, and whole-cell extract was prepared, and chromatin was sonicated with a Biorupter™ sonicator (Diagenode, Denville, NJ) to fragments from approximately 200 to 500 bp and then incubated with antibody specifically reactive to H4 acetylated at lysines K5, K8, K12, and K16 (pan-acetylation) (catalog #04-557, Upstate Biotechnology/Millipore, Billerica, MA), or antibody specifically reactive to H3 acetylated at K9 and K14 (catalog #39140, Active Motif, Carlsbad, CA) and immunoprecipitation performed. The cross-linking was reversed and ChIP and input control samples purified and amplified with WGA2 GenomePlex Complete Whole Genome Amplification (WGA) kit from Sigma-Aldrich Corporation (St. Louis, MO). Custom-designed tiling microarrays were generously provided by NimbleGen Inc. (Madison, WI) (http://www.nimblegen.com). Each microarray contained 710,907 probes that permitted up to four matches within the genome. Of all probes, approximately 20,000 matched the Ch5 sequences. The probes were in situ synthesized 50-mers with an average probe spacing of 35 bp on each strand tiled in an unbiased fashion across the entire genome. Empty features on the array were filled with randomly generated probes that had G + C content and length comparable to the C. albicans probes as controls for non-specific binding.
Array hybridizations were performed by Roche NimbleGen. Each array was hybridized with a mixture of ChIP-selected DNA fragments labeled with Cy5 and control input DNA from the same strain labeled with Cy3. We obtained the data from two independent experiments each for H4 and H3 acetylation. Signal intensities were scanned and normalized, and the ratio of ChIP DNA/Input DNA for either Sor125(55) or 3153A and difference between log2 ratios Sor125(55)/Input DNA and log2 ratios 3153A/Input DNA for either H4 or H3 acetylation were determined and are presented independently for each repeat in Additional file 6: Table S2. Raw data are available at GEO with the accession number GSE81684. An analysis was performed using an algorithm written in Python and plotted as the position of the probes on each chromosome in the reference strain SC5314, as annotated in genomic assambly 21 in CGD, versus the averaged log2 ratio Sor125(55) minus log2 ratio 3153A. Thus, the graphs reflect the difference in acetylation with data plotted above or below the X-axis reflecting increased or decreased acetylation in aneuploid cells compared to that in disomic parental cells, respectively. Thus, a score of +1 reflects a twofold increase in acetylation at a particular locus in the mutant compared to the parental strain. To minimize random noise on the plots, which obscured real effects due to the high probe density, log2 ratio differences were counted as significant and plotted only if the following criteria were met: mean log2 ratio difference of 0.2 units or greater (in the same direction) over three consecutive probes and p < 0.1 for all three consecutive probes. The use of three consecutive probes for this analysis is based on the fact that the average size of the immunoprecipitated DNA fragments was similar to the size of a genomic region covered by three probes. Thus, each dot corresponds to the location of three consecutive probes on the chromosome that satisfied a high stringency statistical filter.
Western blot analysis
Candida albicans cells were seeded on YPD plates (3000 cfu/plate) and incubated at 37 °C. Cells were collected in wash buffer containing 20 mM Tris, pH 8, 0.1 M NaCl, 0.5 mM dithiothreitol, 5 mM EDTA and washed three times in this buffer. Cells were suspended in lysis buffer containing 20 mM Tris, pH 8, 0.1 M NaCl, 0.1% NP-40, 0.5 mM dithiothreitol, 5 mM EDTA, 10 mM Sodium butyrate, and Protease Inhibitor Mini Tablets (Thermo Scientific, Rockford, IL), then microglass beads (Biospec Products, Bartlesville, OK) added, and cell lysed in a BeadBeater (Mini-Beadbeater-1, Biospec Products) at 20 s duration with 10 ~ 1-min intervals on ice. The lysed cells were mixed with 0.4 N HCl to a final concentration of 0.2 N, incubated on ice for 30 min with occasional vortexing, and centrifuged at 14,000 rpm for 10 min at 4 °C. Supernatants were collected, and 1/5 volume of 100% trichloroacetic acid was added, and after 30 min of incubation on ice, the samples were centrifuged at 14,000 rpm for 10 min at 4 °C and supernatants were discarded. The pellets were resuspended with ice-cold acetone containing 0.05 N HCl and centrifuged at 14,000 rpm for 10 min at 4 °C. The pellets were rinsed with ice-cold acetone lacking HCl twice more than resuspended with 20 mM Tris, pH 8.
Histone preparations were divided into 1 µg samples and were separated on a series of 15% SDS-PAGE gels and then transferred to PVDF membrane (0.2-µm pore size, Thermo Scientific) for Western blots; thus, H4 pan-acetylation and total H4 blots were determined for same histone preparation with the same amount of histone H4. Each Western blot analysis was conducted from three independent cell cultures. The membranes were probed with anti-histone H4, anti-pan-acetylated H4, anti-histone H4acK5, anti-histone H4acK8, anti-histone H4acK12, or anti-histone H4acK16 antibody (catalog ##39270, 39244, 39584, 39173, 39166, or 39168, respectively, Active Motif, Carlsbad, CA) followed by the incubation with ALP-labeled secondary antibody (anti-rabbit IgG linked to alkaline phosphatase, ImmunoReagents, Inc, Raleigh, NC) and detected by chemifluorescence (ECF substrate; GE Healthcare, Piscataway, NJ, USA). Fluorescence signals were detected using Molecular Imager Gel Doc XR + system (Bio-Rad, Hercules, CA), and the band densities and background corrections were quantified by Image Lab software (Bio-Rad). Acetylation levels were obtained as a density value of each histone H4 acetylation divided by density of H4. Then, acetylation levels of mutant versus parent were calculated. Data were subjected to statistical analysis (Student’s t test).
open reading frame
contour-clamped homogenous electrophoretic field
pulse-field gel electrophoresis
Rustchenko E. Chromosome instability in Candida albicans. FEMS Yeast Res. 2007;7:1–11.
Rustchenko E. Specific chromosome alterations of Candida albicans: mechanisms for adaptation to pathogenicity. In: Nombela C, Cassel GH, Baquero F, Gutierrez-Fuentes JA, editors. Evolutionary biology of bacterial and fungal pathogens. Washington: ASM Press; 2008. p. 197–212.
Yang F, Kravets A, Bethlendy G, Welle S, Rustchenko E. Chromosome 5 monosomy of Candida albicans controls susceptibility to various toxic agents, including major antifungals. Antimicrob Agents Chemother. 2013;57:5026–36.
Yang F, Zhang L, Wakabayashi H, Myers J, Jiang Y, Cao Y, Jimenez-Ortigosa C, Perlin DS, Rustchenko E. Tolerance to caspofungin in Candida albicans is associated with at least three distinctive mechanisms that govern expression of FKS Genes and cell wall remodeling. Antimicrob Agents Chemother. 2017;61:e00071-17. doi:10.1128/AAC.00071-17.
Kwon-Chung KJ, Chang YC. Aneuploidy and drug resistance in pathogenic fungi. PLoS Pathog. 2012;8:e1003022.
Ford ChB, Funt JM, Abbey D, Issi L, Guiducci C, Martinez DA, Delorey T, Li BY, White ThC, Cuomo Ch, Rao RP, Berman J, Thompson DA, Regev A. The evolution of drug resistance in clinical isolates of Candida albicans. eLIFE. 2014. doi:10.7554/eLife.00662.
Kravets A, Qin H, Ahmad A, Bethlendy G, Gao Q, Rustchenko E. Widespread occurrence of dosage compensation in Candida albicans. PLoS ONE. 2010;5:e10856.
Kravets A, Yang F, Bethlendy G, Sherman F, Rustchenko E. Adaptation of Candida albicans to growth on sorbose via monosomy of chromosome 5 accompanied by duplication of another chromosome carrying a gene responsible for sorbose utilization. FEMS Yeast Res. 2014;14:708–13.
Suwunnakorn S, Wakabayashi H, Rustchenko E. Chromosome 5 of human pathogen Candida albicans carries multiple genes for negative control of caspofungin and anidulafungin susceptibility. Antimicrob Agents Chemother. 2016;60:7457–67.
Kabir M, Ahmad A, Greenberg J, Wang Y-K, Rustchenko E. Loss and gain of chromosome 5 controls growth of Candida albicans on sorbose due to dispersed redundant negative regulators. Proc Natl Acad Sci USA. 2005;102:12147–52.
Ahmad A, Kravets A, Rustchenko E. Transcriptional regulatory circuitries in the human pathogen Candida albicans involving sense-antisense interactions. Genetics. 2012;190:537–47.
Hallacli E, Akhtar A. X chromosomal regulation in flies: when less is more. Chromosome Res. 2009;17:603–19.
Eisen A, Utley RT, Nourani A, Allard S, Schmidt P, Lane WS, Lucchesi JC, Côté J. The yeast NuA4 and Drosophila MSL complexes contain homologous subunits important for transcription regulation. J Biol Chem. 2001;276:3484–91.
Doyon Y, Côté J. The highly conserved and multifunctional NuA4 HAT complex. Curr Opin Genet Dev. 2004;14:147–54.
Doyon Y, Selleck W, Lane WS, Tan S, Côté J. Structural and functional conservation of the NuA4 histone acetyltransferase complex from yeast to humans. MCB. 2004;24:1884–96.
Wang X, Chang P, Ding J, Chen J. Distinct and redundant roles of the two MYST histone acetyltransferases Esa1 and Sas2 in cell growth and morphogenesis of Candida albicans. Eucaryot Cell. 2013;12:438–49.
Lu Y, Su Ch, Mao X, PalaRaniga P, Liu H, Chen J. Efg1-mediated recruitment of NuA4 to promoters is required for hypha-specific Swi/Snf binding and activation in Candida albicans. Mol Biol Cell. 2008;19:4260–72.
Janbon G, Sherman F, Rustchenko E. Appearance and properties of l-sorbose-utilizing mutants of Candida albicans obtained on a selective plate. Genetics. 1999;153:653–64.
Rustchenko EP, Curran TM, Sherman F. Variations in the number of ribosomal DNA units in morphological mutants and normal strains of Candida albicans and in normal strains of Saccharomyces cerevisiae. J Bacteriol. 1993;175:7189–99.
Rustchenko E. Candida albicans adaptability to environmental challenges by means of specific chromosomal alterations. In: Pandalai SG, editor. Recent research developments in bacteriology, vol. 1. Trivandrum: Transworld Research Network; 2003. p. 91–102.
Lopez da Rosa J, Kaufman PD. Chromatin-mediated Candida albicans virulence. Biochim Biophys Acta. 2012;1819:349–55.
Sellam A, Askew C, Epp E, Lavoi H, Whiteway M, Nantel A. Genome-wide mapping of the coactivator Ada2p yields insight into the functional roles of SAGA/ADA complex in Candida albicans. Mol Biol Cell. 2009;20:2389–400.
Mitchell L, Lambert JP, Gerdes M, Al-Madhoun AS, Skerjanc IS, Figeys D, Baetz K. Functional dissection of the NuA4 histone acetyltransferase reveals its role as a genetic hub and that Esf1 is essential for complex integrity. Mol Cell Biol. 2008;28:2244–56.
Chittuluru JR, Chaban Y, Monnet-Saksouk J, Carrozza M, Sapountzi V, Selleck W, Huang J, Utley RT, Cramet M, Allard S, Cai G, Workman JL, Fried MG, Tan S, Côté J, Asturias FJ. Structure and nucleosome interaction of the yeast NuA4 and piccolo-NuA4 histone acetyltransferase complexes. Nat Struct Mol Biol. 2011;18:1196–203.
Hose J, Mun Yong C, Sardi M, Wang Z, Newton MA, Gasch AP. Dosage compensation can buffer copy-number variation in wild yeasts. eLIFE. 2015. doi:10.7554/eLife.05462.001.
Davis DA, Bruno VM, Loza L, Filler SG, Mitchell AP. Candida albicans Mds3p, is a conserved regulator of pH responses and virulence identified through insertional mutagenesis. Genetics. 2002;162:1573–81.
Janbon G, Sherman F, Rustchenko E. Monosomy of a specific chromosome determines l-sorbose utilization: a novel regulatory mechanism in Candida albicans. Proc Natl Acad Sci USA. 1998;95:5150–5.
Sherman F. Getting started with yeast. Methods Enzymol. 2003;350:3–41.
Rustchenko-Bulgac E. Variations of Candida albicans electrophoretic karyotypes. J Bacteriol. 1991;173:6586–96.
Ahmad A, Kabir MA, Kravets A, Andaluz E, Larriba G, Rustchenko E. Chromosome instability and unusual features of some widely used strains of Candida albicans. Yeast. 2008;25:433–48.
Drouin S, Robert F. Genome-wide location analysis of chromatin-associated proteins by ChIP on CHIP: controls matter. 2015; in press. https://www.researchgate.net/publication/268401136_Genome-wide_Location_Analysis_of_Chromatin-associated_Proteins_by_ChIP_on_CHIP_Controls_Matter
ER, MB, and JH conceived and designed the experiments and wrote the manuscript. HW, GB, and AK performed the experiments. SLW, ChT, and HW analyzed the data. All authors read and approved the final manuscript.
We thank the Tag-Module collection in the University of Toronto and the FGSC for deletion strains. We thank Cheeptip Benyajati for the critical reading of the manuscript.
The authors declare that they have no competing interests.
Availability of data and materials
ChIP-Chip data (Accession Number GSE81684) from this study have been deposited into NCBI GEO http://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?acc=GSE81684.
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All authors read and approved the manuscript.
Ethics approval and consent to participate
This work was supported in part by the University of Rochester Funds to ER, as well as partially supported by National Institutes of Health Grants Number 1R01AI110764 to ER, R01GM52426 to JH, and R01DK070687 to MB.
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The original version of this article was revised. The author name Jeffrey J. Hayes was missing the middle initial.
A correction to this article is available online at https://doi.org/10.1186/s13072-017-0161-1.
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Wakabayashi, H., Tucker, C., Bethlendy, G. et al. NuA4 histone acetyltransferase activity is required for H4 acetylation on a dosage-compensated monosomic chromosome that confers resistance to fungal toxins. Epigenetics & Chromatin 10, 49 (2017) doi:10.1186/s13072-017-0156-y
- Candida albicans
- H4 and H3 acetylation
- Chromosome 5 monosomy