Linkage mapping of yeast cross protection connects gene expression variation to a higher-order organismal trait

Gene expression variation is extensive in nature, and is hypothesized to play a major role in shaping phenotypic diversity. However, connecting differences in gene expression across individuals to higher-order organismal traits is not trivial. In many cases, gene expression variation may be evolutionarily neutral, and in other cases expression variation may only affect phenotype under specific conditions. To understand connections between gene expression variation and stress defense phenotypes, we have been leveraging extensive natural variation in the gene expression response to acute ethanol in laboratory and wild Saccharomyces cerevisiae strains. Previous work found that the genetic architecture underlying these expression differences included dozens of “hotspot” loci that affected many transcripts in trans. In the present study, we provide new evidence that one of these expression QTL hotspot loci affects natural variation in one particular stress defense phenotype—ethanol-induced cross protection against severe doses of H2O2. A major causative polymorphism is in the heme-activated transcription factor Hap1p, which we show directly impacts cross protection, but not the basal H2O2 resistance of unstressed cells. This provides further support that distinct cellular mechanisms underlie basal and acquired stress resistance. We also show that Hap1p-dependent cross protection relies on novel regulation of cytosolic catalase T (Ctt1p) during ethanol stress in a wild oak strain. Because ethanol accumulation precedes aerobic respiration and accompanying reactive oxygen species formation, wild strains with the ability to anticipate impending oxidative stress would likely be at an advantage. This study highlights how strategically chosen traits that better correlate with gene expression changes can improve our power to identify novel connections between gene expression variation and higher-order organismal phenotypes.


Introduction
A fundamental question in genetics is how individuals with extremely similar genetic makeups can have dramatically different characteristics. One hypothesis is that a small number of regulatory polymorphisms can have large effects on gene expression, leading to the extensive phenotypic variation we see across individuals. In fact, gene expression variation is hypothesized to underlie the extensive phenotypic differences we see between humans and chimpanzees despite >98% DNA sequence identity [1,2]. This hypothesis is supported by numerous examples of gene expression variation affecting higher-order organismal traits.
While gene expression variation is pervasive, there is often a lack of obvious phenotypic change associated with differentially expressed genes. This can occur for a variety of reasons. First, a large fraction of expression variation has been postulated to be evolutionarily neutral with no effect on organismal fitness [28][29][30]. Second, co-regulation of genes that share the same upstream signaling network and transcription factors can lead to genes whose expression differences correlate with phenotype but are not truly causative. Finally, some gene expression differences may truly affect phenotype, but only under specific conditions. For example, the predictive power of expression quantitative trait loci (eQTL) mapping studies on higher-order phenotypes can be poor unless multiple environments are considered [31]. Similarly, tissuerestricted eQTLs are more likely to map to known disease-associated loci identified from GWAS than non-tissue-restricted eQTLs [32,33].
Thus, a major challenge for connecting gene expression variation to downstream effects on higher-order traits is the choice of which conditions and traits to examine. To this end, we have been leveraging natural variation in the model eukaryote Saccharomyces cerevisiae, and a phenotype called acquired stress resistance. Many studies have shown a poor correlation between genes that respond to stress and their importance for surviving stress [34][35][36][37][38][39][40][41][42][43]. Thus, we and others have argued that the role of stress-activated gene expression is not to survive the initial insult, but instead protects cells from impending severe stress through a phenomenon called acquired stress resistance [44,45]. Acquired stress resistance (sometimes referred to as "induced tolerance" or the "adaptive response") occurs when cells pretreated with a mild dose of stress gain the ability to survive an otherwise lethal dose of severe stress. Notably, acquired stress resistance can occur when the mild and severe stresses are the same (same-stress protection) or across pairs of different stresses (cross protection). This phenomenon has been observed in diverse organisms ranging from bacteria to higher eukaryotes including humans [44][45][46][47][48][49][50]. The specific mechanisms governing acquisition of higher stress resistance are poorly understood, but there are wide reaching implications. In humans, ischemic preconditioning (transient ischemia followed by reperfusion-i.e. mild stress pretreatment followed by severe stress) may improve outcomes of cardiovascular surgery [51-54], while transient ischemic attacks ("mini-strokes") may protect the brain during massive ischemic stroke [55][56][57]. Thus, understanding the genetic basis of acquired stress resistance in model organisms holds promise for mitigating the effects of stress in humans.
A previous study found that a commonly used S288c lab strain is unable to acquire further ethanol resistance when pretreated with a mild dose of ethanol [44]. We found this phenotype to be surprising, considering the unique role ethanol plays in the life history of Saccharomyces yeast, where the evolution of aerobic fermentation gave yeast an advantage over ethanol-sensitive competitors [58]. Because ethanol is a self-imposed stress that induces a robust stress response [59-63], we expected that ethanol should provoke acquired stress resistance in wild yeast strains. Indeed, this turned out to be the case, with the majority of tested wild strains acquiring resistance to severe ethanol following a mild ethanol treatment [45]. Furthermore, this phenotype correlated with extensive differences in the transcriptional response to acute ethanol stress in the lab strain when compared to a wild vineyard (M22) and wild oak (YPS163) strain (>28% of S288c genes were differentially expressed at an FDR of 0.01) [45,64]. We performed linkage mapping of S288c crossed to a wild vineyard strain (M22) and wild oak strain (YPS163), and observed numerous "hotspots" where the same eQTL loci affect the expression of a large number of transcripts (anywhere from 10-500 transcripts per hotspot) [64].
In the present study, we provide new evidence that one of these eQTL hotspot loci affects natural variation in acquired stress resistance, namely the ability of ethanol to cross protect against oxidative stress in the form of hydrogen peroxide. The causative polymorphism is in the heme-activated transcription factor Hap1p, which we show directly impacts cross protection, but not the basal resistance of unstressed cells. Finally, we show that the Hap1p effect is mediated through novel regulation of cytosolic catalase T (Ctt1p) during ethanol stress in wild strains. This study highlights how strategically chosen traits that are better correlated with gene expression changes can improve our power to identify novel connections between gene expression variation and higher-order organismal phenotypes.

The genetic basis of natural variation in yeast cross protection
We previously found that an S288c-derived lab strain was unable to acquire further ethanol resistance when pretreated with a mild dose of ethanol, in contrast to the vast majority of~50 diverse yeast strains [45]. In addition to the S288c strain's acquired ethanol resistance defect, ethanol also failed to cross protect against other subsequent stresses [44,65]. In nature, wild yeast cells ferment sugars to ethanol, and then shift to a respiratory metabolism that generates endogenous reactive oxygen species [66][67][68]. Thus, we hypothesized that ethanol might cross protect against oxidative stress in wild yeast strains. We tested this hypothesis by assessing whether mild ethanol treatment would protect a wild oak strain (YPS163) from severe oxidative stress in the form of hydrogen peroxide (H 2 O 2 ). Cross protection assays were performed by exposing cells to a mild, sublethal dose of ethanol (5% v/v) for 60 min, followed by exposure to a panel of 11 increasingly severe doses of H 2 O 2 (see Materials and Methods). Confirming the observations of Berry and Gasch [44], ethanol failed to cross protect against H 2 O 2 in S288c, and in fact slightly exacerbated H 2 O 2 toxicity (Fig 1). In contrast, ethanol strongly cross protected against H 2 O 2 in YPS163 (Fig 1).
The inability of ethanol to induce acquired stress resistance in S288c correlates with thousands of differences in ethanol-dependent gene expression in comparison to wild strains that can acquire ethanol resistance [45,64]. In light of this observation, and the known dependency of cross protection on stress-activated gene expression changes [44], we hypothesized that differences in cross protection against H 2 O 2 by ethanol may be linked to differential gene expression. To test this, we performed quantitative trait loci (QTL) mapping using the same mapping population as our original eQTL study that mapped the genetic architecture of ethanol-responsive gene expression [64]. Specifically, we conducted QTL mapping of both basal and acquired H 2 O 2 resistance in 43 F 2 progeny of S288c crossed with YPS163 (see Materials and Methods). While we found no significant QTLs for basal H 2 O 2 resistance, we did find a significant QTL peak on chromosome XII that explained 38% of the variation in cross protection (Fig 2). It is unlikely that our failure to detect a chromosome XII QTL for basal H 2 O 2 resistance was due to a lack of statistical power, because two independent basal H 2 O 2 resistance QTL studies using millions of S288c x YPS163 F 2 segregants also found no significant associations at this locus [69,70]. Additionally, we estimated the heritability of phenotypic variation in basal resistance to be 0.79, which is slightly above the median value estimated by Bloom and colleagues for 46 yeast traits [71], and is only moderately lower than the heritability for cross protection (0.92).

Fig 1. Natural variation in ethanol-induced cross protection against H 2 O 2 . (A)
A representative acquired H 2 O 2 resistance assay is shown. S288c (lab strain-DBY8268) and YPS163 (wild oak strain) were exposed to 5% ethanol or mock (5% water) pretreatment for 60 min, washed, exposed to 11 doses of severe H 2 O 2 for 2 hr, and then plated to score viability. (B) A single survival score was calculated from the viability at all H 2 O 2 doses (see Materials and Methods). Each plot shows the mean and standard deviation of 4 independent biological replicates. The replicates for mock-treated YPS163 all had the same tolerance score and thus zero standard deviation (see S1 Lastly, the shape of the distribution of phenotypes in the F 2 were markedly different between basal and acquired H 2 O 2 resistance, with basal resistance showing a transgressive segregation pattern and acquired resistance showing a continuous distribution (S1 Fig). Altogether, these results suggest that the genetic basis of natural variation in acquired stress resistance is distinct from the basal resistance of unstressed cells (see Discussion).
The significant QTL for cross protection was located near a known polymorphism in HAP1, a heme-dependent transcription factor that controls genes involved in aerobic respiration [72][73][74], sterol biosynthesis [75][76][77], and interestingly, oxidative stress [77,78]. S288c harbors a known defect in HAP1, where a Ty1 transposon insertion in the 3' end of the gene's coding region has been shown to reduce its function [79]. In fact, we previously hypothesized that the defective HAP1 allele was responsible for the inability of S288c to acquire further resistance to ethanol. However, a YPS163 hap1Δ strain was still fully able to acquire ethanol resistance, despite notable differences in the gene expression response to ethanol in the mutant [45]. Likewise, despite previous studies implicating Hap1p as a regulator of oxidative stress defense genes [77,78], HAP1 is apparently dispensable for same-stress acquired H 2 O 2 resistance [47]. These observations suggest that the molecular mechanisms underlying various acquired stress resistance phenotypes can differ, even when the identity of the secondary stress is the same.

A role for HAP1 in ethanol-induced cross protection against severe H 2 O 2
Because we previously implicated HAP1 as a major ethanol-responsive eQTL hotspot affecting over 100 genes, we hypothesized that ethanol-induced cross protection against H 2 O 2 may depend upon Hap1p-regulated genes. However, it was formally possible that HAP1 was merely linked to the truly causal polymorphism. To distinguish between these possibilities, we generated deletion mutations in the YPS163 background for every non-essential gene within the 1.5-LOD support interval of the QTL peak (encompassing IFH1 -YCS4). Of the 36 mutants tested, two showed significantly and highly diminished acquired H 2 O 2 resistance (Fig 3 and S2  Fig), hap1Δ and top3Δ (encoding DNA topoisomerase III). To determine whether different alleles of HAP1 and/or TOP3 were responsible for natural variation in acquired H 2 O 2 resistance, we applied an approach called reciprocal hemizygosity analysis [80], where the TOP3 and HAP1 alleles were analyzed in an otherwise isogenic S288c-YPS163 hybrid background (see Fig 4A for a schematic). In each of the two reciprocal strains, one allele of the candidate gene was deleted, producing a hybrid strain containing either the S288c or YPS163 allele in single copy (i.e. hemizygous for TOP3 or HAP1). While we found only mild allelic effects for TOP3, the effects of different HAP1 alleles were striking (Fig 4B and 4C). The hybrid strain containing the HAP1 YPS163 allele showed full cross protection, while the strain containing the HAP1 S288c allele showed none. Thus, we examined the effects of HAP1 on acquired H 2 O 2 resistance further. Intriguingly, we found that the YPS163 hap1Δ mutant was unaffected for acquired H 2 O 2 resistance when mild H 2 O 2 or mild NaCl were used as mild stress pretreatments (Fig 5), suggesting that Hap1p plays a distinct role in ethanol-induced cross protection (see Discussion). Deletions of all nonessential genes within the 1.5-LOD support interval of the chromosome XII QTL peak were constructed in JL111 (YPS163 MATa haploid) background and tested for defects in acquired H 2 O 2 resistance. Each plot shows the mean and standard deviation of 2 independent biological replicates, with the exception of the JL111 control (35 replicates). The replicates for several strains all had the same tolerance score and thus zero standard deviation (see S1 Table for raw numerical data). Asterisks represent acquired H 2 O 2 resistance that was significantly lower than wild-type YPS163 ( Ã P < 0.001, one-way ANOVA). https://doi.org/10.1371/journal.pgen.1007335.g003 Finally, we performed allele swap experiments to examine the effects of the different HAP1 alleles in the original parental backgrounds. We introduced only the Ty element from HAP1 S288c into the YPS163 HAP1 gene, and observed a loss of acquired H 2 O 2 resistance similar to the YPS163 hap1Δ strain (Fig 6). We next tested whether repair of the defective hap1 allele in S288c could restore cross protection. Surprisingly, S288c repaired with HAP1 YPS163 was largely unable to acquire further H 2 O 2 resistance (Fig 6). This additional layer of genetic complexity suggests that S288c harbors additional polymorphisms that affect cross protection. To determine whether this was due to allelic variation in TOP3, the only other locus showing a difference in acquired H 2 O 2 resistance, we genotyped each of the segregants at both the HAP1 and TOP3 loci. We identified two segregants with both the HAP1 YPS163 and TOP3 YPS163 alleles that were nonetheless unable to acquire further resistance (S3 Fig, S1 Table). These data, along (A) Schematic of reciprocal hemizygosity analysis. Each block represents a gene, and each hybrid strain contains a single-copy deletion of hap1 or top3, and a single copy of the respective S288c (lab) or YPS163 (oak) allele. (B) Representative acquired H 2 O 2 resistance assays for wild-type YPS163, the YPS163-S288c hybrid, and the reciprocal hemizygotes. (C) Each survival score plot shows the mean and standard deviation of biological triplicates. Asterisks represent significant differences in acquired resistance between denoted strains ( ÃÃ P < 0.01, ÃÃÃ P < 0.001, ns = not significant (P > 0.05), t-test). https://doi.org/10.1371/journal.pgen.1007335.g004 with the continuous distribution of F 2 phenotypes (S1 Fig), is consistent with other loci outside of the chromosome XII QTL peak contributing to variation in acquired H 2 O 2 resistance. Moreover, the causative alleles at these loci are apparently masked in YPS163-S288c hybrids that fully acquire H 2 O 2 resistance, suggesting that they are recessive (see Discussion). We also noted during the genotyping that a small number of segregants contained the HAP1 S288c (or TOP3 S288c ) allele but were still able to acquire further H 2 O 2 resistance (S3 Fig and S1 Table), suggesting that HAP1 function is conditionally necessary in certain genetic backgrounds. To determine whether this was due to a unique genetic background for YPS163, we deleted HAP1 in three additional wild strains. A wild oak (YPS1000) and wild vineyard (M22) strain showed defects in acquired H 2 O 2 resistance similar to that of the YPS163 hap1Δ strain, while a wild coconut (Y10) strain showed a very slight defect (S4 Fig). Altogether, these results are consistent with HAP1 being necessary for ethanol-induced cross protection against H 2 O 2 in some genetic backgrounds, including those of several wild strains, but not others (see Discussion).

Fig 5. HAP1 is not required for acquired H 2 O 2 resistance following mild H 2 O 2 or mild NaCl pretreatments.
Cultures of wild-type YPS163 and the YPS163 hap1Δ mutant were split and exposed to either 0.4 mM H 2 O 2 , 0.4 M NaCl, or a mock (media only) treatment for 60 min, washed, exposed to 11 doses of severe H 2 O 2 for 2 hr, and then plated to score viability. The survival scores across each of the 11 doses are plotted as the mean and standard deviation of biological triplicates.

HAP1 affects catalase expression and peroxidase activity during ethanol stress
Because Hap1p is a transcription factor, we hypothesized that acquired H 2 O 2 resistance relied on Hap1p-dependent expression of a stress protectant protein. We reasoned that the putative stress protectant protein should have the following properties: i) a biological function consistent with H 2 O 2 detoxification or damage repair, ii) reduced ethanol-responsive expression in S288c versus YPS163, iii) be a target gene of the HAP1 eQTL hotspot, and iv) possess evidence of regulation by Hap1p.
We first focused on CTT1, since it is both necessary for NaCl-induced cross protection against H 2 O 2 in S288c [84], and sufficient to increase H 2 O 2 resistance when exogenously overexpressed in S288c [85]. We deleted CTT1 in the YPS163 background, and found that ethanol-induced cross protection against H 2 O 2 was completely eliminated (Fig 8). The complete lack of cross protection in the ctt1Δ mutant suggests that other peroxidases cannot compensate for the lack of catalase activity under this condition. Next, because CTT1 was part of the HAP1 eQTL hotspot (Fig 7C, plotted using the data described in [64]), we tested whether the S288c HAP1 allele reduced CTT1 expression during ethanol stress. To do this, we performed qPCR to measure CTT1 mRNA induction following a 30-minute ethanol treatment (i.e. the peak ethanol response [45]). Consistent with our previous microarray data [45,64], we saw lower induction of CTT1 by ethanol in S288c relative to YPS163 (Fig 9A). Moreover, we saw dramatically reduced induction of CTT1 in a YPS163 hap1Δ mutant compared to the wild-type YPS163 control (Fig 9A). Further support that HAP1 is causative for reduced CTT1 expression was provided by performing qPCR in the HAP1 reciprocal hemizygotes, where we found that the HAP1 S288c allele resulted in significantly reduced CTT1 induction compared to the HAP1 YPS163 allele (Fig 9A).
To determine whether the differences in CTT1 induction across strain backgrounds also manifested as differences in each strain's ability to detoxify H 2 O 2 , we measured in vitro peroxidase activity in cell-free extracts. We compared in vitro peroxidase activity in extracts from unstressed cells and cells exposed to ethanol stress for 60 minutes (i.e. the same pre-treatment time that induces acquired H 2 O 2 resistance (see Materials and Methods)). For wild-type YPS163, ethanol strongly induced peroxidase activity, and this induction was completely dependent upon CTT1 (Fig 9B). Mirroring CTT1 gene expression patterns, the induction of peroxidase activity was reduced in a YPS163 hap1Δ mutant. Additionally, reciprocal hemizygosity analysis provided further support that lack of HAP1 function results in decreased peroxidase activity, as the hybrid containing the HAP1 S288c allele showed significantly reduced peroxidase activity following ethanol stress compared to the hybrid containing the HAP1 YPS163 allele ( Fig 9B). Notably, the hybrid containing the HAP1 YPS163 allele had lower CTT1 induction and in vitro peroxidase activity following ethanol shock than wild-type YPS163, despite equivalent levels of acquired H 2 O 2 resistance in the strains. These results suggest that HAP1 may play additional roles in acquired H 2 O 2 resistance beyond H 2 O 2 detoxification, depending upon the genetic background (see Discussion). Interestingly, S288c showed no induction of peroxidase activity upon ethanol treatment, despite modest induction of the CTT1 transcript. This result is reminiscent of Ctt1p regulation during heat shock in the S288c background, where mRNA levels increase without a concomitant increase in protein levels [84]. Thus, in addition to strain-specific differences in CTT1 regulation at the RNA level, there are likely differences in regulation at the level of translation and/or protein stability.

Discussion
In this study, we leveraged extensive natural variation in the yeast ethanol response to understand potential connections between gene expression variation and higher-order organismal Overlap between genes that were HAP1 eQTL hotspot targets from [64], genes with defective induction in S288c vs. YPS163 from [64], and direct targets of HAP1 identified via ChIP experiments compiled from [81]. (B) Descriptions of the eight genes that overlapped for all three criteria. (C) Previous eQTL mapping of the yeast ethanol response (newly plotted here using data described in [64]), implicated HAP1 as causative for natural variation in CTT1 induction levels during ethanol stress.   Peroxidase activity measured in cell-free extracts in either mock-treated or ethanol-stressed cells. The plots indicate the mean and standard deviation of biological triplicates (mRNA) or quadruplicates (peroxidase activity). Asterisks represent significant differences in CTT1 mRNA induction or peroxidase activity between denoted strains ( Ã P < 0.05, ÃÃ P < 0.01, paired t-test).
https://doi.org/10.1371/journal.pgen.1007335.g009 [84]. Thus, we hypothesized that phenotypic variation in acquired stress resistance may be linked to natural variation in stress-activated gene expression. Our results provide a compelling case study in support of this notion-namely that a polymorphism in the HAP1 transcription factor affects natural variation in acquired H 2 O 2 resistance, but not the basal H 2 O 2 resistance of unstressed cells. Forward genetic screens have shown that the genes necessary for basal and acquired resistance are largely non-overlapping [34,36,84], suggesting that mechanisms underlying basal and acquired stress resistance are distinct. We provide further genetic evidence to support this model. YPS163 hap1Δ mutants and the hybrid carrying the HAP1 S288c allele had strong acquired H 2 O 2 defects, but no differences in their basal H 2 O 2 resistance (Figs  4 and 6). Moreover, the YPS163 hap1Δ mutant was affected only when ethanol was the mild pretreatment, and was able to fully acquire H 2 O 2 resistance following mild H 2 O 2 or mild NaCl (Fig 5). These results suggest that the mechanisms underlying acquired resistance differ depending upon the mild stress that provokes the response. Further dissection of the mechanisms underlying acquired stress resistance will provide a more integrated view of eukaryotic stress biology.
Our results reveal a new role for Hap1p in cross protection against H 2 O 2 that has been lost in the S288c lab strain. We propose that a major mechanism underlying ethanol-induced cross protection against H 2 O 2 is the induction of cytosolic catalase T (Ctt1p), and that in the YPS163 background, Hap1p is necessary for proper induction of CTT1 during ethanol stress. We based this mechanism on the following observations. First, over-expression of CTT1 in S288c is sufficient to induce high H 2 O 2 resistance [85]. Second, a YPS163 ctt1Δ mutant cannot acquire any further H 2 O 2 resistance following ethanol pre-treatment (Fig 8), suggesting that no other antioxidant defenses are able to compensate under this condition. Lastly, the defect in cross protection for the YPS163 hap1Δ mutant correlates with reduced CTT1 expression and peroxidase activity during ethanol stress (compare Figs 6 and 9). How Hap1p is involved in the regulation of CTT1 during ethanol stress remains an open question, but we offer some possibilities. Hap1p is activated by heme, thus promoting transcription of genes involved in respiration, ergosterol biosynthesis, and oxidative stress defense including CTT1 [75,76,78,82]. Because heme biosynthesis requires oxygen, Hap1p is an indirect oxygen sensor and regulator of aerobically expressed genes [74,75,86]. There is currently no evidence that heme levels are affected by ethanol stress, nor is there evidence that Hap1p is "super-activating" under certain conditions. Thus, we disfavor a mechanism of induction caused solely by Hap1p activation. Instead, we favor a mechanism where Hap1p interacts with other transcription factors at the CTT1 promoter during ethanol stress, leading to full CTT1 induction. One possibility that we favor is recruitment of the general stress transcription factor Msn2p, which plays a known role in acquired stress resistance [44,45]. We previously showed that a YPS163 msn2Δ mutant had no induction of CTT1 mRNA during ethanol stress [45], suggesting that Msn2p was an essential activator for CTT1 under this condition. The CTT1 promoter region contains three Msn2p DNA-binding sites, two of which are~100-bp away from the Hap1p binding site. Hap1p binding to the CTT1 promoter could help recruit Msn2p during ethanol stress, possibly through chromatin remodeling that increases accessibility of the Msn2p binding sites as proposed by Elfving and colleagues [87].
What is the physiological role of Hap1p-dependent induction of CTT1 during ethanol stress? One possibility is that regulation tied to the heme-and oxygen-sensing role of Hap1p ensures that CTT1 induction only occurs under environmental conditions where reactive oxygen species (ROS) are most likely to be encountered-namely stressful conditions that are also aerobic. In the context of ethanol stress, aerobic fermentation would lead to subsequent respiration of the produced ethanol and simultaneous ROS production. Under these conditions, CTT1 induction leading to ethanol-mediated cross protection against ROS would likely confer a fitness advantage. On the other hand, during stressful yet anoxic conditions, Ctt1p and other ROS-scavenging proteins are likely unnecessary. Furthermore, because heme is not synthesized during anoxic conditions [74], Hap1p would fail to induce CTT1 and other genes encoding non-essential heme-containing proteins. This may improve fitness by conserving energy used for biosynthesis and by redirecting limited heme to more essential heme-containing proteins.
The S288c lab strain has long been known to possess a defective HAP1 allele [79]. Apparently, the defective allele arose relatively recently, as only S288c contains a HAP1 Ty1 insertion out of over 100 sequenced strains [88,89]. The lack of HAP1 function in S288c could be due to relaxation of selective constraint, though others have argued in favor of positive selection for reduced ergosterol biosynthetic gene expression [90,91]. Regardless, the loss of ethanolinduced acquired H 2 O 2 resistance is likely a secondary effect of the loss of Hap1p function. Intriguingly, we did find that two (non-S288c) domesticated yeast strains also lack ethanolinduced cross protection against H 2 O 2 (S5 Fig), suggesting that phenotypic differences in acquired stress resistance may differentiate domesticated versus wild yeast. Because environmental stresses are likely encountered in combination or sequentially [92], acquired stress resistance is likely an important phenotype in certain natural ecological settings. Future studies directed at understanding differences in acquired stress resistance phenotypes in diverse wild yeast strains may provide unique insights into the ecology of yeast.
While our QTL mapping identified HAP1 as the major effector of cross protection, we note that additional complexity remains unexplained. Notably, despite the strong cross protection defect in the YPS163 hap1Δ mutant, some residual cross protection persists that is absent in S288c (Fig 6). Intriguingly, the residual cross protection is also absent in the hybrid carrying the HAP1 S288c allele, suggesting the involvement of other genes depending upon the genetic background (Fig 4B and 4C). It is known that yeast strains with respiratory defects have increased ROS sensitivity [93,94], potentially due to increased programmed cell death [95]. It is possible that reduced respiratory activity and concomitant ROS sensitivity in strains lacking HAP1 is exacerbated by genetic interactions with other alleles.
The lack of cross protection in S288c and the HAP1 S288c hybrid correlates with the lack of inducible peroxidase activity following ethanol pretreatment in those strains. The lack of inducible peroxidase activity in S288c despite modest induction of CTT1 mRNA could be due to translational regulation, which is supported by the observation that while mild heat shock induces CTT1 mRNA, protein levels remain nearly undetectable [84]. Strikingly, the hybrid carrying the HAP1 YPS163 allele still cross protects despite levels of CTT1 mRNA induction and peroxidase activity that are lower than in the YPS163 hap1Δ strain that is unable to acquire further resistance (Fig 9). These data suggest that HAP1 plays an additional role in ethanolinduced cross protection beyond H 2 O 2 detoxification by Ctt1p. Moreover, the continuous distribution of the cross protection phenotype in the segregants (S1 Fig) and the results of allele swap experiments (Fig 6) strongly implicate other genes and processes in this complex trait. Specifically, the lack of complementation by the HAP1 YPS163 allele in the S288c background suggests that additional loci in S288c render HAP1 necessary but not sufficient for cross protection in this background. Moreover, our genotyping of the segregants at HAP1 revealed a small number that still possessed cross protection in the absence of functional HAP1 (S3 Fig  and S1 Table), suggesting that HAP1 is dispensable in certain genetic backgrounds. We examined the effects of hap1Δ mutations in other wild strain backgrounds and found two additional strains with a strong HAP1 requirement and a third strain with at most a mild HAP1 effect (S4 Fig). This result, as well as those from other recent studies [96][97][98], suggests that these types of genetic background effects are likely the rule rather than the exception. Future high resolution mapping experiments will be necessary to identify and characterize the source of these genetic background effects.
Gene expression variation is extensive in nature and is hypothesized to be a major driver of higher-order phenotypic variation. However, there are inherent challenges to connecting gene expression variation to higher-order organismal traits. Hundreds to thousands of genes are often differentially expressed across individuals, so identifying which particular transcripts exert effects on fitness is difficult. By studying acquired stress resistance-a phenotype better correlated with stress-activated gene expression changes-we were able to uncover a novel connection between gene expression variation and an organismal trait.

Strains and growth conditions
Strains and primers used in this study are listed in S2 and S3 Tables, respectively. The parental strains for QTL mapping were YPS163 (oak strain) and the S288c-derived DBY8268 (lab strain; referred to throughout the text as S288c). The construction of the S288c x YPS163 QTL mapping strain panel (44 F 2 progeny) is described in [99] (kindly provided by Justin Fay). Genotypes for the strain panel are listed in S4 Table. During the course of analyzing HAP1 genotypes, we found one segregant (YS.15.2) to be a mixed population, so it was removed from subsequent analyses. Deletions in the BY4741 (S288c) background were obtained from Open Biosystems (now GE Dharmacon), with the exception of hap1 (whose construction is described in [45]). Deletions were moved into haploid MATa derivatives of DBY8268, M22, and YPS163 by homologous recombination with the deletion::KanMX cassette amplified from the appropriate yeast knockout strain [100]. Homozygous hap1Δ strains of YPS1000 and Y10 were generated by moving the hap1Δ::KanMX allele from the BY4741 background into the strains, followed by sporulation and tetrad dissection. All deletions were verified by diagnostic PCR. DBY8268 containing a wild-type HAP1 allele from YPS163 was constructed in two steps. First, the MX cassette from the hap1Δ::KanMX deletion was replaced with a URA3MX cassette, selecting for uracil prototrophy. Then, URA3 was replaced with wild-type HAP1 from YPS163 (amplified using primers 498-bp upstream and 1572-bp downstream of the HAP1 ORF), while selecting for loss of URA3 on 5-fluoroorotic acid (5-FOA) plates. Deletions and repair of HAP1 were confirmed by diagnostic PCR (see S3 Table for primer sequences). YPS163 containing a HAP1 S288c allele was constructed by first inserting a KanMX cassette into S288c 117-bp downstream of the Ty element to create JL1032. We then amplified and transformed the Ty element into YPS163 using primers that annealed 103-bp upstream of the Ty element and 177-bp downstream of the KanMX cassette, generating JL1069. Diploid strains for HAP1 and TOP3 reciprocal hemizygosity analysis were generated as follows. The hemizygote containing the wild-type S228c HAP1 allele (JL580) was generated by mating JL140 (YPS163 MATa hoΔ::HygMX hap1Δ::KanMX) to JL506 (DBY8268 MATα ho ura3 hap1). The hemizygote containing the wild-type YPS163 allele (JL581) was generated by mating JL112 (YPS163 MATα hoΔ::HygMX HAP1) to JL533 (DBY8268 MATa ho ura3 hap1Δ::KanMX). The hemizygote containing the wild-type S288c TOP3 allele (JL1107) was created by mating JL1066 (YPS163 MATa hoΔ:: HygMX top3Δ::KanMX) to BY4742 (MATα TOP3). The hemizygote containing the wild-type YPS163 allele (JL1106) was created by mating JL1121 (BY4741 MATa top3Δ::KanMX) to JL112 (YPS163 MATα hoΔ::HygMX TOP3). All strains were grown in batch culture in YPD (1% yeast extract, 2% peptone, 2% dextrose) at 30˚C with orbital shaking (270 rpm).

HAP1 and TOP3 genotyping
To identify possible promoter polymorphisms, the HAP1 promoters of the DBY8268 (JL505), YPS163 (JL111), and S288c HAP1 YPS163 (JL975) strains were amplified using primers that anneal 1091-bp upstream and 134-bp downstream of the HAP1 start codon. PCR products were purified with a PureLink PCR cleanup kit (Invitrogen) and sequenced by Sanger Sequencing (Eurofins Genomics) using a primer that anneals 498-bp upstream of the HAP1 start codon. Sequences were aligned to the S288c and YPS163 reference sequences using SnapGene v4.1 (GSL Biotech). This verified the presence of a 1-bp indel within a poly-A stretch that differs between S288c and YPS163. The S288c HAP1 YPS163 (JL975) strain contains the YPS163 HAP1 promoter sequence. Additionally, the YPS163 strain containing the HAP1 S288c was constructed to only contain the Ty element and not the S288c promoter polymorphism.
The HAP1 allele of each segregant for the QTL mapping panel was genotyped by differential PCR analysis where the same forward primer (HAP1 int 3' F) was paired with two different reverse primers. One primer (Ty R) anneals specifically to the Ty element, yielding an 856-bp product when amplifying the S288c allele. The second primer (HAP1 3' end R) anneals 3' to the Ty element of HAP1 S288c , yielding a 570-bp product for HAP1 YPS163 and a 6.5-kb product for HAP1 S288c . Each segregant was genotyped using both sets of primer pairs, and only one segregant (YS.15.2) appeared to contain both HAP1 alleles. Subsequent analysis of multiple colonies verified that YS.15.2 was a mixed population, and thus it was removed it from all subsequent analyses.
The TOP3 alleles of S288c and YPS163 contain two non-synonymous SNPs at nucleotide positions 1,398 and 1,422. Segregant genotypes at TOP3 were determined by analyzing restriction fragment length polymorphisms. TOP3 was amplified using primers (TOP3 up F and TOP3 down R) that anneal~500-bp upstream and downstream of the open reading frame, generating a 2.9-kb product. PCR products were digested with either 1) PstI, which cuts at position 1,248 only within the TOP3 YPS163 ORF allele yielding 1.7-and 1.2-kb products, or (2) KflI, which cuts at position 1,155 only within the TOP3 S288c yielding 1.6-and 1.3-kb products. Genotypes for HAP1 and TOP3 are listed in S1 Table.

Cross protection assays
Cross-protection assays were performed as described in [44] with slight modifications. Briefly, 3-4 freshly streaked isolated colonies (<1 week old) were grown overnight to saturation, subcultured into 6 ml fresh media, and then grown for at least 8 generations (>12 h) to mid-exponential phase (OD 600 of 0.3-0.6) to reset any cellular memory of acquired stress resistance [85]. Each culture was split into two cultures and pretreated with YPD media containing either a single mild "primary" dose or the same concentration of water as a mock-pretreatment control. Primary doses consisted of 5% v/v ethanol, 0.4 M NaCl, or 0.4 mM H 2 O 2 . Thereafter, mock and primary-treated cells were handled identically. Following 1-hour pretreatment at 30˚C with orbital shaking (270 rpm), cells were collected by mild centrifugation at 1,500 x g for 3 min. Pelleted cells were resuspended in fresh medium to an OD 600 of 0.6, then diluted 3-fold into a microtiter plate containing a panel of severe "secondary" H 2 O 2 doses ranging from 0.5-5.5 mM (0.5 mM increments; 150 μl total volume). Microtiter plates were sealed with air-permeable Rayon films (VWR), and cells were exposed to secondary stress for 2 hours at 30˚C with 800 rpm shaking in a VWR symphony Incubating Microplate Shaker. Four μl of a 50-fold dilution was spotted onto YPD agar plates and grown 48 h at 30˚C. Viability at each dose was scored using a 4-point semi-quantitative scale to score survival compared to a no-secondary stress (YPD only) control: 100% = 3 pts, 50-90% = 2 pts, 10-50% = 1 pt, or 0% (3 or less colonies) = 0 pts. An overall H 2 O 2 tolerance score was calculated as the sum of scores over the 11 doses of secondary stress. Raw phenotypes for all acquired stress resistance assays can be found in S1 Table. A fully detailed acquired stress protocol has been deposited to protocols.io under doi dx.doi.org/10.17504/protocols.io.g7sbzne. Statistical analyses were performed using Prism 7 (GraphPad Software).

QTL mapping and heritability estimates
Phenotyping of the QTL mapping strain panel for basal and acquired H 2 O 2 resistance was performed in biological duplicate. Because cross-protection assays on the entire strain panel could not all be performed at the same time, we sought to minimize day-to-day variability. We found that minor differences in temperature and shaking speed affected H 2 O 2 resistance; as a result, we used a digital thermometer and tachometer to ensure standardization across experiments. Moreover, we found that differences in handling time were a critical determinant of experimental variability. To minimize this source of variability, all cell dilutions were performed quickly using multichannel pipettes, and no more than two microtiter plates were assayed during a single experiment. To ensure that replicates on a given day were reproducible, we always included the YPS163 wild-type parent as a reference.
Single mapping scans were performed using Haley-Knott regression [101] implemented through the R/QTL software package [102]. Genotype probabilities were estimated at every cM across the genome using the calc.genoprob function. Significant LOD scores were determined by 100,000 permutations that randomly shuffled phenotype data (i.e. strain labels) relative to the genotype data. The maximum LOD scores for the permuted scans were sorted, and the 99 th percentile was used to set the genome-wide FDR at 1%. This resulted in LOD cutoffs of 3.07 for QTL mapping of basal H 2 O 2 resistance, and 4.24 for acquired H 2 O 2 resistance.
Broad-sense heritability (H 2 ) was estimated from the segregant data as described in [71] using a random-effects ANOVA model implemented through the lmer function in the lme4 R package [103]. H 2 was estimated using the equation represents the genetic variance due to the effects of segregrant, and s 2 E represents the residual (error or environmental) variance. The proportion of variance explained by a QTL was estimated using the equation 1 À 10 ðÀ 2 n ÃLODÞ , where n represents the number of segregants.

Quantitative PCR of CTT1 expression and cellular peroxidase assays
Induction of CTT1 by ethanol was assessed by real-time quantitative PCR (qPCR) using the Maxima SYBR q-PCR Master Mix (Thermo Fisher Scientific) and a Bio-Rad CFX96 Touch Real-Time PCR Detection System, according to the manufacturers' instructions. Cells were grown to mid-exponential phase (OD 600 of 0.3-0.6) as described for the cross-protection assays. Cells were collected by centrifugation at 1,500 x g for 3 minutes immediately prior to the addition of 5% v/v ethanol (unstressed sample) and 30 minutes post-ethanol treatment, which encompasses the peak of global expression changes to acute ethanol stress [45]. Cell pellets were flash frozen in liquid nitrogen and stored at -80˚C until processed. Total RNA was recovered by hot phenol extraction as previously described [104], and then purified with a Quick-RNA MiniPrep Plus Kit (Zymo Research) including on-column DNase I treatment. cDNA synthesis was performed as described [104], using 10 μg total RNA, 3 μg anchored oligo-dT (T20VN), and SuperScript III (Thermo Fisher Scientific). One ng cDNA was used as template for qPCR with the following parameters: initial denaturation at 95˚C for 3 minutes followed by 40 cycles of 95˚C for 15 seconds and 55˚C annealing and elongation for 1 minute. Cq was determined using regression analysis, with baseline subtraction via curve fit. The presence of a single amplicon for each reaction was validated by melt curve analysis. The average of two technical replicates were used to determine relative CTT1 mRNA abundance via the ΔΔCq method [105], by normalizing to an internal control gene (ERV25) whose expression is unaffected by ethanol stress and does not vary in expression between S288c and YPS163 [45]. Primers for CTT1 and ERV25 were designed to span~200 bp in the 3' region of each ORF (to decrease the likelihood of artifacts due to premature termination during cDNA synthesis), and for gene regions free of polymorphisms between S288c and YPS163 (see S3 Table for primer  sequences). Three biological replicates were performed and statistical significance was assessed via a paired t-test using Prism 7 (GraphPad Software). For peroxidase activity assays, mid-exponential phase cells were collected immediately prior to and 60 minutes post-ethanol treatment, to assess peroxidase activity levels during the induction of cross protection. Cells were collected by centrifugation at 1,500 x g for 3 minutes, washed twice in 50 mM potassium phosphate buffer, pH 7.0 (KP i ), flash frozen in liquid nitrogen, and then stored at -80˚C until processed. For preparation of whole cell extracts, cells were thawed on ice, resuspended in 1 ml KP i buffer, and then transferred to 2-ml screw-cap tubes for bead beating. An equal volume (1 ml) of acid-washed glass beads (425-600 micron, Sigma-Aldrich) was added to each tube. Cells were lysed by four 30-second cycles of bead beating in a BioSpec Mini-Beadbeater-24 (3,500 oscillations/minute, 2 minutes on ice between cycles). Cellular debris was removed by centrifugation at 21,000 x g for 30 minutes at 4˚C. The protein concentration of each lysate was measured by Bradford assay (Bio-Rad) using bovine serum albumin (BSA) as a standard [106]. Peroxidase activity in cellular lysates was monitored as described [107], with slight modifications. Briefly, 50 μg of cell free extract was added to 1 ml of 15 mM H 2 O 2 in KP i buffer. H 2 O 2 decomposition was monitored continuously for 10 minutes in Quartz cuvettes (Starna Cells, Inc.) at 240 nm (ε 240 = 43.6 M -1 cm -1 ) using a Spectra-Max Plus Spectrophotometer (Molecular Devices). One unit of catalase activity catalyzed the decomposition of 1 μmol of H 2 O 2 per minute. For each sample, results represent the average of technical duplicates. To assess statistical significance, four biological replicates were performed and significance was assessed via a paired t-test using Prism 7 (GraphPad Software).  Fig. HAP1 is necessary for acquired H 2 O 2 resistance in some wild strains. Survival score plots indicating the mean and standard deviation of at least biological triplicates. The replicates for mock-treated Y10 all had the same tolerance score and thus zero standard deviation (see S1 Table for raw numerical data). Asterisks represent significant differences in acquired resistance between denoted strains ( Ã P < 0.05, ÃÃ P < 0.01, ÃÃÃ P < 0.001, ns = not significant (P > 0.05), t-test). The replicates for ethanol-treated YJM627 all had the same tolerance score and thus zero standard deviation (see S1