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Distinct adaptive mechanisms drive recovery from aneuploidy caused by loss of the Ulp2 SUMO protease


In response to acute loss of the Ulp2 SUMO-specific protease, yeast become disomic for chromosome I (ChrI) and ChrXII. Here we report that ChrI disomy, which creates an adaptive advantage in part by increasing the dosage of the Ccr4 deadenylase, was eliminated by extended passaging. Loss of aneuploidy is often accompanied by mutations in essential SUMO-ligating enzymes, which reduced polySUMO-conjugate accumulation. The mRNA levels for almost all ribosomal proteins increase transiently upon initial loss of Ulp2, but elevated Ccr4 levels limit excess ribosome formation. Notably, extended passaging leads to increased levels of many small nucleolar RNAs (snoRNAs) involved in ribosome biogenesis, and higher dosage of three linked ChrXII snoRNA genes suppressed ChrXII disomy in ulp2Δ cells. Our data reveal that aneuploidy allows rapid adaptation to Ulp2 loss, but long-term adaptation restores euploidy. Cellular evolution restores homeostasis through countervailing mutations in SUMO-modification pathways and regulatory shifts in ribosome biogenesis.


Environmental changes induce many acute and long-term adaptive cellular responses. Mammals have diverse adaptive mechanisms for stress resistance, such as immune responses to pathogens or hormone-mediated homeostatic processes1,2. At the cellular level, acute changes in the local microenvironment, such as changes of pH or temperature, oxidative stress, or nutrient limitation, may induce programmed cell death or trigger adaptive changes that include gene mutation, aneuploidy, changes in gene expression or epigenetic alterations3,4,5. Aneuploidy alters the dosage of genes on the extra chromosome(s), often amplifying a particular gene(s) required to increase cell survival3. In some cases, rapidly activated mechanisms that restore homeostasis are superseded by more robust, long-term adaptations6. For instance, specific aneuploidies are rapidly induced by heat or high pH; however, persistent exposure to the same stresses eventually leads to gene mutation and alterations in transcription, instead of aneuploidy7, which is usually deleterious to cell fitness but is a common feature of cancer cells8.

The yeast Saccharomyces cerevisiae has been a useful model for studying evolutionary processes under laboratory conditions, providing insights into adaptive genetic mechanisms in microbial populations subject to specific growth conditions9. Adaptations often involve genomic sequence polymorphisms, including single-nucleotide variations, insertions, deletions, and other structural variations, as well as large copy number variants and aneuploidy10,11,12. Such studies revealed that many genome modifications contribute to species diversification, evolution, and adaptation4,13,14.

The small ubiquitin-like modifier (SUMO) protein is a conserved post-translational modifier that regulates a host of proteins in eukaryotic cells15. The C-terminus of mature SUMO is first activated by the heterodimeric SUMO-activating enzyme E1 (Aos1/Uba2), which then transfers the SUMO to the SUMO-conjugating enzyme E2 (Ubc9). Finally, SUMO is transferred to specific substrates with the aid of an E3 SUMO ligase (Siz1, Siz2, or Mms21). SUMO-substrate deconjugation in yeast is catalyzed by the SUMO proteases Ulp1 and Ulp216. While much is known about Ulp1, most molecular functions of Ulp2 remain unclear. Ulp2 has particularly high activity towards polySUMO chains, and it preferentially localizes to the nucleus. Its loss results in a pleiotropic mutant phenotype including defects in cell growth; sensitivity to heat, DNA damage or aberrant spindle formation; and high rates of chromosome and plasmid loss17. Recently, we reported that acute loss of Ulp2 leads to aneuploidy, specifically, a double disomy of chromosome I (ChrI) and ChrXII, an adaptive mechanism that compensates for a severely dysregulated SUMO system18. Increased dosage of two ChrI genes, CLN3, encoding a G1 cyclin, and CCR4, encoding the catalytic deadenylase subunit of the Ccr4-Not complex, were shown to drive the ChrI disomy18,19.

Yeast SUMO pathway mutants show abnormal formation of 60s pre-ribosomes20. In normal ribosome biogenesis, the 35s ribosomal RNA (rRNA) precursor is processed into the mature 25s, 18s, and 5.8s rRNAs; the 5s rRNA is independently transcribed21. The 60s subunit contains 46 proteins and the 25s, 5.8s, and 5s rRNAs, while the 40s subunit comprises the 18s rRNA and 33 proteins. Ribosome biogenesis involves many rRNA modifications that are catalyzed by small nucleolar ribonucleoprotein complexes (snoRNPs) composed of small nucleolar RNAs (snoRNAs) and nucleolar proteins22. The 77 snoRNAs in S. cerevisiae fall into three classes: box C/D snoRNAs responsible for 2′-O-ribose methylation, box H/ACA snoRNAs mediating pseudouridylation, and the NME1 snoRNA that participates in rRNA cleavage. SUMO is also involved in snoRNP biogenesis through its conjugation to Nop58 and Nhp2, core proteins of both Box C/D and H/ACA snoRNPs23.

Here, we report that the ChrI and ChrXII aneuploidy triggered by acute loss of Ulp2 is completely lost within 500 generations of growth. RNA-seq experiments reveal that many RP gene transcripts are substantially increased in response to the potentially lethal effects of acute ULP2 gene loss. However, following extended culture, RP mRNAs subside to wild-type (WT) levels while more than half of the snoRNAs are significantly upregulated. Provision of high levels of a polycistronic snoRNA cluster, consisting of SNR61, SNR55, and SNR57 from ChrXII, suppresses the enhanced expression of RPs in cells lacking ULP2. Linking the two disomies in nascent ulp2Δ cells, the ChrI duplication drives an increase in Ccr4 binding at snoRNA and rDNA loci, preventing their overexpression. The ulp2Δ cells also acquire mutations in genes encoding the SUMO-ligating enzymes Ubc9 or Uba2/Aos1 during laboratory evolution. The point mutations in these essential genes inhibit the accumulation of high-molecular-weight (HMW) polySUMO conjugates caused by loss of Ulp2. This inhibition of HMW polySUMO is paralleled by suppression of ulp2Δ growth defects. Taken together, our data suggest that ribosome biogenesis is an essential target of SUMO regulation, and its perturbation by loss of the polySUMO-selective Ulp2 protease is compensated by distinct short-term and long-term adaptive mechanisms. Mutations in essential SUMO-conjugation pathway components are a recurrent feature of long-term adaptation as well. This remarkable genetic malleability in response to disruption of SUMO-protein conjugation dynamics is likely relevant to other pathways that link cell growth and division to essential post-translational modifications.


ChrI disomy of ulp2Δ cells is lost after extended culture

We first explored how quickly aneuploidy is established. For this we developed an improved inducible AID* degron-tagged ULP2 construct in which the degradation of the mRNA can also be induced through a neomycin-regulated self-cleaving hammerhead ribozyme in the 3′-UTR (Supplementary Fig. 1). We observed that a single ChrI disomy was preferentially generated in cells after depletion of Ulp2, although it took many days in culture. Although we could no longer detect the Ulp2 protein even at the first timepoint (2 days), it is likely that there was still a very low level present that limited the transition to the aneuploid state. Potentially, the transition occurs in a step-wise fashion, with ChrI disomy needed before ChrXII duplication can occur.

We had reported that ChrXII, but not ChrI, disomy was eliminated after 100 generations of continuous culture of ulp2Δ cells with repeated cycles of dilution and outgrowth in fresh medium18. To determine if the ChrI disomy would eventually also be lost during laboratory evolution, we monitored the relative copy number of ChrI at various points after the establishment of the ulp2Δ null state (Fig. 1a, b). We previously analyzed copy number for up to 250 cell generations and had not seen loss of ChrI18. By contrast, the extra copy of ChrI in ulp2Δ cells had disappeared by 500 generations. The more rapid elimination of extra ChrXII compared to ChrI, and the eventual loss of both extra copies, was verified by an independent experiment (Supplementary Fig. 2). Yeast ulp2Δ mutants are impaired in cell-cycle progression and chromosome segregation as well as growth17,24. The growth and cell-cycle defects were also fully suppressed in the long-term adapted cells (Fig. 1c, e), which was paralleled by a (partial) reduction in HMW SUMO conjugates (Fig. 1d). Hence, adaptation to loss of Ulp2 leads to a transient aneuploidy, which after culturing for many generations results in reversion to euploidy, nearly WT growth and cell-cycle progression, and reduced accumulation of the HMW SUMO conjugates typical of ulp2Δ cells.

Fig. 1

Aneuploidy of ulp2Δ cells can be reversed by laboratory evolution. a Scheme for creation of nascent ulp2Δ cells and their subsequent passaging. The ulp2Δ cells containing YCplac33-ULP2 were streaked on SD + FOA plates twice sequentially to evict the YCplac33-ULP2 plasmid, and they were then transformed either with YCplac33-ULP2 or YCplac33. Cells grew for ~50 generations (50 G) during these procedures. For long-term passaging, cells were grown until saturation and then diluted 1:120 in fresh YPD (6.9 generations per dilution). This process was repeated daily. b Chromosome copy number of ulp2Δ cells with the indicated plasmids was monitored by qPCR assay at the indicated number of generations. Copy number was determined relative to WT (MHY500 + YCplac33) cells. Chromosome copy number between 50 and 250 generations were monitored previously18, and the data are included here. c Growth of the indicated ulp2Δ strains at 50G and 500G. After spotting cells in fivefold serial dilutions, the YPD plates were incubated for 2 days at 30 °C. d Immunoblot analysis of sumoylated proteins in extracts prepared from the strains in c. Anti-Pgk1 blotting was used to verify the equal loading. Asterisks indicate reintroduced YCplac33-ULP2. The stacking gel (bracket) and molecular size standards are indicated. e Flow cytometry of DNA content of the strains from c. 1C and 2C indicate unreplicated DNA (haploid) and replicated DNA (diploid), respectively

High RP levels in ulp2Δ normalize after multiple generations

Aneuploidy is often associated with responses to stress; the duplicated chromosomes encode genes whose increased levels appear to counteract detrimental effects of the stress3,25. Gene expression imbalances resulting from aneuploidy, however, carry a fitness cost26,27. Aneuploidy may serve as a rapid stopgap response that can be superseded by more sustainable adaptations that somehow counter the stress7. Because aneuploidy disappeared and growth and cell-cycle defects were mitigated by evolving ulp2Δ cells over long periods (Fig. 1), we asked if the evolved strain had acquired any genetic changes.

Genome-wide gene expression profiles of the evolved ulp2Δ cells were analyzed by RNA-seq. In these comparisons, the ulp2Δ cells either carried a WT ULP2 plasmid or empty vector and were passaged for 50 or 500 generations (G). Expression of many transcripts was significantly different among the indicated strains (Supplementary Figs. 3a and 4). Differentially expressed genes and their changes relative to expression in the WT control strain (ulp2Δ + YCplac33-ULP2, 50 G) are shown in Fig. 2a. In nascent ulp2 null cells (ulp2Δ+ YCplac33, 50 G), ~80% of the significant changes (twofold or more) involved increases in transcript levels (Fig. 2a and Supplementary Fig. 3b). Genes encoding ribosomal proteins (RPs) and ribosome biogenesis factors were heavily enriched among the genes with strong increases in expression (Fig. 2c (middle) and Supplementary Data 1). Among 136 genes encoding yeast ribosomal subunits, 130 were significantly upregulated in the ulp2 null mutant. By contrast, high expression of RP genes was no longer seen in ulp2 null cells after long-term culture at 30˚C in YPD medium (ulp2Δ+ YCplac33, 500 G; Fig. 2c right). Indeed, these long-term adapted ulp2Δ cells had much more overlap in their upregulated transcripts with WT cells than with the nascent ulp2Δ strain (Fig. 2b, c). As predicted from the RNA-seq results, enhanced levels of ribosomal protein Rpl32 in nascent ulp2Δ cells were observed, and this returned to control levels after 500 generations. (Fig. 2d).

Fig. 2

Analysis of genome-wide gene expression of ulp2Δ cells during passaging. a Volcano plots displaying differentially expressed genes in the indicated strains as compared to MHY1379 (ulp2Δ+ YCplac33-ULP2) at 50G. The y-axis is the mean of the negative logarithm of the P-values, and the x-axis corresponds the log2 fold change value. Green and magenta dots denote genes significantly changed if the fold change was >2 (|fold changes| > 2) and <2, respectively, and gray dots denote genes with statistically insignificant changes. b Venn diagram of genes with significantly increased expression (green dots shown in a). c Gene Ontology (GO) enrichment analysis of the genes displayed in b. Bar diagrams indicate the fold-enrichment of categories of biological process to the genome using GO data from SGD and PANTHER. The genes used in GO biological process are listed in Supplementary Data 1. d Immunoblot analysis of the Rpl32 ribosomal protein in extracts from the indicated strains. Anti-Pgk1 blotting was used to verify equal loading. Arrowhead, Rpl32 protein. e A percentage graph of snoRNA gene expression that was significantly changed in ulp2Δ+ YCplac33 at 500G. Genes were binned by fold change (χ). NC, no change. f Growth assay of the indicated strains. After spotting cells in fivefold serial dilutions, plates were incubated at 30 °C for 2 (YPD) or 5 days (YPD + Rap). Asterisks indicate reintroduced YCplac33-ULP2. Rap, 10 μg/ml rapamycin. g qRT-PCR analysis of ribosomal protein genes, RPL12B and RPS18B, in ulp2Δ cells transformed with yeast genomic library plasmids including the indicated snoRNA genes. Expression was measured relative to WT cells (MHY1379) containing empty vector (pGP564). Data were normalized to ACT1 expression. The error bars indicate the standard deviation (SD) from three independent RNA preparations. Asterisks represent statistically significant differences determined by pairwise comparisons between ulp2Δ cells with empty vector (–) and each snoRNA plasmid using a two-tailed Student’s t-test (*P < 0.05; **P < 0.01). h Immunoblot analysis of the Rpl32 protein in ulp2Δ cells containing plasmids with the indicated snoRNA genes, performed as in 2d

Earlier genome-wide analysis of SUMO modifications in yeast revealed that SUMO preferentially localizes to genes involved in translation, such as tRNA and RP genes28, and both RPs and ribosome biogenesis factors undergo SUMOylation29. Interestingly, sumoylation of the Rap1 transcription factor cooperates with the target of rapamycin complex 1 (TORC1) kinase pathway to promote transcription of genes encoding RPs28. We therefore tested whether the elevated RP transcripts seen in nascent ulp2Δ cells could potentially overcome inhibition of TORC1 by rapamycin, (Fig. 2f). Despite growing more poorly on rich medium alone (YPD), the nascent ulp2Δ strain grew better than the matched WT strains on rapamycin (at 50G; top two rows). After long-term passage, all the strains grew better on the drug, although not as robustly as the nascent ulp2 null strain. These data are consistent with the model that TORC1 and sumoylated Rap1 function in parallel to promote transcription of RP genes28.

We found that sumoylated Rap1 is a substrate of Ulp2 (Supplementary Fig. 5a). Association of Rap1 with RP genes was not significantly affected by loss of Ulp2 (Supplementary Fig. 5b), consistent with data suggesting sumoylation of Rap1 functions downstream of Rap1 binding to RP promoters28. The elevated levels of SUMO-conjugated Rap1 in ulp2Δ may therefore help drive RP gene transcription and rapamycin resistance.

Numerous snoRNAs are elevated in high-passage ulp2Δ cells

Increased levels of several categories of transcripts, such as those for fatty acid beta-oxidation and ammonium transport, were seen in both ulp2Δ cells containing a ULP2 plasmid (WT) and those with an empty vector after 500 generations (Fig. 2c). These might reflect a general response to long-term growth under these laboratory conditions. A much more specific response of long-term adapted ulp2 null cells was the increase of many snoRNAs, which are critical for rRNA modification (Fig. 2c, right). Of 77 annotated snoRNAs, expression of over half (42) was significantly elevated, compared with WT (Fig. 2e and Supplementary Data 2). The snoRNAs contribute both to the processing of the pre-rRNA into 18s, 5.8s, and 28s rRNAs, and to methylation and pseudouridylation of rRNA30. Novel snoRNA functions are also being uncovered, including some important for oncogenesis and different stress responses31,32,33,34. Notably, a multiple myeloma-associated snoRNA, ACA11, downregulates transcription of RP genes35.

Although we could not simultaneously upregulate dozens of snoRNAs, as observed in high-passage ulp2Δ cells, we could test whether increased levels of specific snoRNA gene(s) could ameliorate any of the ulp2 mutant defects that characterize low-passage cultures. Yeast 2-µm genomic library plasmids containing one or more snoRNA genes were transformed into WT (MHY1379) cells, and the URA3-marked ULP2 plasmid was then evicted. For these tests, we selected 13 plasmids bearing snoRNAs that displayed comparatively large increases in levels in high-passage ulp2Δ cells (Fig. 2e and Supplementary Data 2). None of the high-copy plasmids rescued the growth impairment, aneuploidy, or accumulation of HMW SUMO-conjugated proteins typical of low-passage ulp2Δ cells (Supplementary Fig. 6). However, plasmids containing certain snoRNA genes suppressed the elevated transcripts of the tested RPL12B and RPS18B RP genes, with eight and five, respectively, of the 13 plasmids suppressing to significant degrees (Fig. 2g). Furthermore, 11 of the 13 plasmids as well as an additional plasmid with three clustered snoRNA genes from ChrXII (see below) reduced excess accumulation of Rpl32 protein upon loss of Ulp2 (Fig. 2h). Whether the identified snoRNAs directly regulate RP expression cannot be inferred from these data, but the inverse correlation in expression between a cohort of snoRNAs and RP genes is supported. Inasmuch as snoRNAs are essential for ribosome formation, it is possible that enhanced ribosome biogenesis under these snoRNA overexpression conditions partially relieves the requirement for higher RP gene expression.

Ulp2 modulates SUMO modification at RP and snoRNA genes

Past studies have implicated mammalian SUMO proteases in numerous transcriptional processes16, but there was no evidence that yeast Ulp2 is directly involved in transcription. To determine whether Ulp2 is recruited to RP or snoRNA genes, we carried out chromatin immunoprecipitation (ChIP) assays using cells with the chromosomal ULP2 gene tagged with a sequence encoding a Flag epitope. We used the Rap1 transcription factor as a positive control as it is known to associate with the RP genes and some snoRNA genes28. The ChIP analysis indicated that Ulp2 associated with the promoter and coding sequence (CDS) of both RP and snoRNA genes (Fig. 3a); the protein deacetylase Hst3 and the transcriptional repressor Nrg2, whose genes were significantly downregulated in ulp2Δ cells after extensive passaging, were not associated with these genes. These data suggest that Ulp2 could be directly involved in transcription of these gene classes.

Fig. 3

Ulp2 localizes to ribosomal protein and snoRNA genes and affects local sumoylation. a Chromatin immunoprecipitation (ChIP) analysis using IgG-Sepharose or anti-Flag agarose beads and strains expressing TAP-tagged Rap1, Hst3, or Nrg2 or Flag-tagged Ulp2. Real-time PCR signals at promoter (Pro) and coding sequence (CDS) regions of indicated genes were quantitated and normalized to an internal background control and the input DNA. The error bars indicate the SD calculated from two independent chromatin preparations. b Occupancy of Smt3 at the indicated genes was determined in the WT and ulp2Δ strains expressing His-tagged Smt3 by ChIP using Ni+2-NTA resin and analyzed as shown in a. The error bars indicate the SD from two independent preparations. c, d qRT-PCR analysis of 18s and 25s rRNA in the indicated strains done as in Fig. 2g. Data were normalized to SPT15 expression. The error bars indicate the SD from two independent RNA samples, and asterisks indicate statistically significant differences (*P < 0.05; **P < 0.01, two-tailed Student’s t-test). e Gene expression analysis of ribosomal protein genes RPL12B and RPS18B and snoRNA genes SNR30 or SNR60 by qRT-PCR assay, performed as in Fig. 2g. Expression was measured relative to WT cells (MHY500). Data were normalized to SPT15 expression. The error bars represent the SD from two independent RNAs, and asterisks indicate statistically significant differences (*P < 0.05, two-tailed Student’s t-test). f Immunoblot analysis of Ccr4-Flag or Not5-Flag in the indicated ulp2Δ strains. Anti-Pgk1 blotting was used to verify equal loading. g ChIP assay using anti-Flag agarose beads in the indicated strains as shown in a. The error bars indicate the SD from two independent experiments. h Proposed model of transcription of genes required for ribosome biogenesis in ulp2Δ cells. RPs, SNRs, and rRNA indicate genes of ribosomal proteins, snoRNAs and ribosomal RNA, respectively. Normally, Ulp2 represses transcription of RP, snoRNA, and rRNA genes, and Ccr4 protein, encoded on ChrI, represses expression of snoRNAs and rRNA but not RPs. Loss of Ulp2 leads to ChrI disomy, and the increased level of ChrI-encoded Ccr4 counters the loss of Ulp2-dependent repression of transcription of snoRNA and rRNA, but not RP, genes

Association of the Ulp2 SUMO protease with chromatin sites would be predicted to decrease local protein sumoylation, as occurs at the RP genes28. We compared levels of yeast SUMO (Smt3) at the RP and snoRNA genes in WT and ulp2Δ cells (Fig. 3b). His6-tagged Smt3 was used for the ChIP analysis. Loss of Ulp2 was associated with increased levels of SUMO/Smt3 in both the promoter and CDS regions at most of the tested loci.

Taken together, our data reveal that Ulp2 associates with RP and snoRNA loci where it limits local accumulation of SUMO (presumably SUMO-conjugated chromatin proteins such as Rap1 or histones). This suggests that Ulp2 has a direct role in the expression of RP and snoRNA genes.

Increased Ccr4 in ulp2Δ limits expression of snoRNA and rRNA

Many rDNA silencing factors are targets of sumoylation, and at least the Net1, Tof2, Cdc14 and Fob1 nucleolar proteins are substrates of Ulp236,37. Ulp2 localizes to rDNA loci, and Ulp2 mutations strongly impair association of Net1, Tof2 and Fob1 with rDNA36, suggesting Ulp2 generally promotes rDNA silencing. We therefore assumed that rRNA levels would be altered in ulp2Δ cells undergoing laboratory evolution; however, rRNA levels were unchanged in cells passaged for 50 or 500 generations (Fig. 3c).

We previously reported that ChrI aneuploidy in ulp2Δ cells is suppressed by increased dosage of two ChrI genes, one encoding Ccr4, a subunit of the multifunctional Ccr4–Not complex, and the other Cln3, a G1-phase cyclin18. Therefore, raising either Ccr4 or Cln3 levels is sufficient to prevent the ChrI duplication. Notably, the Ccr4-Not complex limits RNA Pol I binding to rDNA loci and inhibits rRNA synthesis38. Moreover, a wide variety of snoRNAs are over-expressed in mutants of the Ccr4-Not complex39,40.

We confirmed that lack of Ccr4 resulted in higher expression of rRNA (18s and 25s), SNR30, and SNR60 (Fig. 3d, e); RP transcript levels were unaffected. The ulp2Δ mutation by itself did not alter expression of these genes, but in a ulp2Δ ccr4Δ strain, these RNAs, and not RP transcripts, appeared to be modestly increased relative to ccr4Δ. Ccr4 protein levels rose sharply as a result of the ChrI disomy in nascent ulp2Δ cells (Fig. 3f); this increase was accompanied by a specific enrichment of Ccr4, but not the Not5 subunit of the Ccr4-Not complex, at snoRNA gene promoters as well as the 35s gene (Fig. 3g).

Taken together, our data and previous results suggest that Ulp2 may generally limit transcription of the RP, snoRNA and rRNA genes, whereas Ccr4 blocks the expression of snoRNA and rRNA genes, but not of RP genes (Fig. 3h, left). Loss of Ulp2 leads to increased Ccr4 as a result of the ChrI disomy, which in turn limits the transcription of snoRNA and rRNA genes (Fig. 3h, right). The net effect is a specific increase in RP expression in incipient ulp2Δ cells.

Exogenous ChrXII snoRNAs suppress the ChrXII ulp2Δ disomy

Next, we screened for genes on ChrXII that could prevent the ChrXII disomy upon ULP2 deletion (Fig. 4a). Each of 135 plasmids containing individual ChrXII fragments41 was transformed into ulp2Δ cells carrying a URA3-marked ULP2 plasmid (MHY1379), and the ULP2 plasmid was then evicted. Ratios of ChrI and ChrXII to ChrIII, a chromosome that is not duplicated in ulp2Δ cells, were analyzed by a qPCR-based ploidy assay (Supplementary Fig. 7).

Fig. 4

Identification of genes on ChrXII suppressing ulp2Δ aneuploidy. a Strategy used to identify specific regions of ChrXII that suppress ulp2Δ aneuploidy. A ulp2Δ/YCplac33-ULP2 strain (MHY1379) was transformed with the indicated pGP564 (LEU2)-based ChrXII library plasmids. Cells were struck on SD–Leu + FOA twice in succession to evict YCplac33-ULP2. After the putative candidate plasmids were selected by qPCR-based aneuploidy assays of ChrI, ChrIII, and ChrXII, the copy number of ChrI, ChrV, ChrVIII, ChrX, and ChrXII was determined in ulp2Δ cells bearing the selected plasmids (b) or plasmids including specific ChrXII fragments (d). b qPCR ploidy assays of ulp2Δ cells with the high-copy plasmids from the first round of selection. Copy number of the five tested chromosomes was normalized to the euploid control strain (MHY1379 + pGP564) and compared with ulp2Δ cells expressing empty pGP564 vector. Error bars indicate the SD calculated from two independent genomic DNA preparations. Asterisks indicate plasmids showing a reduction of ChrXII disomy. c Schematic diagrams of plasmids pGP564-11-b5, pGP564-11-c5, pGP564-11-e11 and pGP564-11-f11. Locations of ORFs (arrows or boxes) and gene names are indicated. Subclones used in d are shown as bars below the ChrXII regions. Full-length genes contained within subclones are listed below the bars. d qPCR ploidy assays of ulp2Δ cells with the high-copy plasmids shown in c. Chromosome copy number was determined as in b. Error bars indicate the SD calculated from two independent experiments. Asterisks denote plasmids showing a loss of ChrXII disomy. e qRT-PCR analysis of RPL12B and RPS18B in ulp2Δ cells containing a plasmid with snoRNAs (11-e11) as in Fig. 2g. The data of (–) is identical with the (–) signal shown in Fig. 2g. The error bars represent the SD from three experiments. f ChIP analysis of Rap1-TAP and Ulp2-Flag strains as in Fig. 2a. The error bars indicate the SD from analyses of two independent chromatin preparations. g SUMO levels measured by ChIP assay in the WT and ulp2Δ strains expressing His-tagged Smt3 (SUMO) as in Fig. 2b. The error bars indicate the SD from two independent samples

Transformants with 22 different library plasmids reduced the ratio of ChrI/ChrIII or ChrXII/ChrIII from 2 to 1, suggesting possible suppression of ulp2Δ aneuploidy. We repeated the ploidy assay on five chromosomes with the candidate plasmids in nascent ulp2Δ cells (Fig. 4b). Four plasmids covering two separate regions of ChrXII continued to suppress disomy of ChrXII but not of ChrI, (Fig. 4b, c). They did not affect the slow growth and accumulation of polySUMO conjugates (Supplementary Fig. 8). To determine the genes within these clones required for suppression of the ulp2Δ aneuploidy, 15 DNA fragments were individually cloned into library vector pGP564 (Fig. 4c), and their effect on ploidy was tested (Fig. 4d). Extra copies of CCW12 or a cluster of snoRNA genes (SNR61, SNR55, and SNR57) specifically prevented the development of the ChrXII disomy. Ccw12 is a mannoprotein important for cell wall integrity, and its cellular level is tightly regulated42,43,44. The possible contribution of Ccw12 to ulp2Δ aneuploidy was not pursued further here.

The three snoRNA genes in the cloned cluster were all C/D box snoRNAs. Besides suppressing the ChrXII disomy, high-copy expression of the cluster suppressed the excess expression of RP genes RPL12B and RPS18B normally observed in nascent ulp2 mutant cells (Fig. 4e); the much higher dosage of these three snRNA genes compared to ChrXII disomy presumably accounts for the suppression of RP transcripts only in the former case. As predicted from Fig. 3a, Ulp2 was directly recruited to both promoter and coding sequences of SNR57 (Fig. 4f), and SUMO levels at these sites increased in ulp2Δ cells (Fig. 4g), suggesting that Ulp2 is involved in the transcription of SNR57 as well as other snoRNA genes. These data support the hypothesis that enhanced levels of snoRNAs help circumvent the cellular stress caused by loss of Ulp2, first through a ChrXII disomy that raises the dosage of these C/D box snoRNAs, and then after many generations, through a broad increase in expression of many snoRNAs, which is linked to suppression of excess RP transcripts.

High-passage ulp2Δ cells acquire adaptive mutations

Cellular mechanisms for adaptation to stress include gene mutation, aneuploidy, and transcriptional or translational changes, depending on the nature and length of the stress3,4. In a previous study, aneuploidies developed under heat or high pH stress were superseded over longer periods by gene mutations and refinements of gene expression presumed to carry lower fitness costs than aneuploidy7. We asked if aneuploid ulp2Δ yeast undergo an analogous evolutionary process using whole genome DNA sequencing (DNA-seq) to identify potential gene mutations arising during repeated cell passaging (Table 1). Mutations were detected in both coding and noncoding DNA sequences; we focused on those predicted to cause changes to protein sequences.

Table 1 Mutations in the original ulp2Δ strains passaged for 500 cell generations

Interestingly, BUB1, MAD3, and BUB3 genes, which are involved in the spindle checkpoint of the cell cycle45, and SPO23 gene, encoding a protein that interacts with meiosis-specific protein Spo146, carried missense mutations in evolved ulp2Δ cells that either continuously carried or had reintroduced the ULP2 plasmid. Although these ulp2Δ strains had a CEN plasmid with the WT ULP2 gene, plasmid instability might reduce Ulp2 expression in these cultures17. This could cause cell-cycle arrest in response to checkpoint activation47, a defect that may be overcome by mutations in the checkpoint genes. The adaptive significance of the Spo23 mutation is unknown.

In the ulp2Δ strain that had been passaged for ~500 generations without ULP2 plasmid (ulp2 null cells), two missense mutations were found (Table 1). One was in IFM1, encoding mitochondrial translation initiation factor 2; this was not investigated further. The other mutation was in UBC9, which codes for the SUMO-conjugating E2 enzyme. The predicted K27N substitution is in an N-terminal domain that contains binding sites for the E1 and E3 enzymes48. Accumulation of polySUMO conjugates in these late-passage cells had attenuated as well (Fig. 1d).

Analysis of ulp2Δ descendants after long-term passaging

To assess the generality of the altered mutant phenotype of evolved ulp2Δ cells observed in Figs. 1 and 2, we grew ten separate ulp2Δ lines from a single nascent ulp2Δ colony and evaluated them after 250 and 500 generations. ChrXII disomy, but not that of ChrI, had disappeared by 250 generations in all the evolved lines, as had their growth defects (Fig. 5a, b), consistent with Fig. 1b, c and our previous report18. After an additional 250 generations, the disomy of ChrI was also eliminated. Analysis by FACS showed the recovery from the initial ulp2Δ cell-cycle defect at both 250 and 500 generations (Fig. 5c). Also, after both 250 and 500 generations, all the ulp2Δ strains showed resistance to high temperature and oxidative stress (Supplementary Fig. 9). Consistent with RNA-seq data obtained from ulp2Δ at 500 generations in Fig. 2, all ten of the high-passaged ulp2Δ strains showed reversion of the RPL12B and RPS18B transcripts to normal levels along with elevated transcripts of snoRNAs, SNR30 and SNR60 (Fig. 5d). Thus, all ulp2Δ strains eventually move away from aneuploidy and adopt alternative adaptive strategies that enhance fitness.

Fig. 5

UBA2 and AOS1 genes are mutated in high-passage ulp2Δ cells. ae qPCR ploidy assays (a), growth assays (b), flow cytometry analysis (c), qRT-PCR analysis of ribosomal protein genes RPL12B and RPS18B and snoRNA genes SNR30 or SNR60 (d), and immunoblot analysis of SUMO-conjugated proteins (e) were performed for ten independently evolved ulp2Δ lines at 250 or 500 generations. Gene expression was measured relative to WT cells (MHY1379) and data were normalized to SPT15 expression in d. The error bars indicate the SD from two experiments. f Schematic of Uba2 protein and list of mutations in ulp2Δ 250G or 500G strains. AD, CD, and UFD indicate adenylation, Cys and ubiquitin-like fold domains, respectively. Positions of the catalytic Cys residue and mutations identified in Table 2 are noted. g ubc9Δ, uba2Δ, or uba2Δ aos1Δ strains carrying a YCplac33 plasmid with UBC9, UBA2, or UBA2 AOS1 were transformed with a pRS315 plasmid expressing WT or the indicated mutant proteins. After shuffling out the URA3-marked plasmids, anti-SUMO immunoblot analysis of cell extracts was performed

As noted earlier, after 500 generations of continual passaging, the original ulp2Δ strain tested no longer accumulated excess SUMO conjugates (Fig. 1d). We also measured SUMO conjugate levels by anti-SUMO immunoblotting in the ten separately evolved ulp2Δ strains after 250 and 500 generations (Fig. 5e). PolySUMO-conjugated proteins significantly declined in five of the strains after 250 generations (strains 3, 4, 8, 9, and 10). After 500 generations, conjugate levels had also declined in strains 1 and 7.

Hence, all of the independently evolved ulp2Δ strains eventually reestablished euploidy and near-normal cell growth and cell-cycle progression, but even after 500 generations, several of the strains still accumulated excess HMW SUMO conjugates, suggesting alternative long-term mechanisms for adapting to Ulp2 loss.

Point mutations in the SUMO E1 enzyme in evolved ulp2Δ

In the original evolved ulp2Δ strain, a mutation in the UBC9 gene had been uncovered (Table 1), presumably because reduced E2 activity suppresses accumulation of polySUMO conjugates. No UBC9 mutations were found in the ten new ulp2Δ strains grown without ULP2 for 250 and 500 generations (Table 2). Since most of the evolved ulp2Δ strains showed reduced accumulation of polySUMO conjugates (Fig. 5e), we checked for mutations in all other genes known to be required for normal SUMO conjugation in vegetative cells, specifically those encoding the E1 (Aos1/Uba2 dimer), E3s (Siz1, Siz2 and Mms21), and SUMO protease Ulp1.

Table 2 Mutations of SUMO enzymes caused by Ulp2 loss during multiple cell generations

Interestingly, we found several missense mutations in UBA2, which encodes the catalytic E1 subunit. All ten strains shared a mutation in the UBA2 ORF, causing a C162S change in the encoded protein (Fig. 5f). This mutation was probably acquired during the original 5-FOA counter-selection to evict the covering ULP2 plasmid because all ten ulp2Δ strains originated from the same colony after growth for ~30 generations on 5-FOA. Additional UBA2 missense mutations were observed in six of the evolved ulp2Δ strains (Fig. 5f). All these ulp2Δ strains expressed a doubly mutated Uba2 and suppressed accumulation of polySUMO conjugates (Fig. 5e). Strain 8, which also suppressed polySUMO-conjugate levels yet had no additional Uba2 mutations, picked up a mutation in Aos1 (E346V). Interestingly, while the uba2-C162S mutation was insufficient to suppress polySUMO-conjugate levels in strains 1 and 7 at 250 generations, the additional Uba2 mutations seen at 500 generations were associated with a strong decrease in conjugate levels. Conversely, three evolved ulp2Δ strains (2, 5, and 6) had no detectable changes in the tested SUMO pathway components, consistent with their continued high levels of polySUMO conjugates (Fig. 5e).

The Uba2 missense mutations occurred throughout the protein (Fig. 5f). Only C162S is located within the domain bearing the catalytic Cys173 residue. The other mutations occur in the adenylation domain (AD) or the ubiquitin-like domain (UFD) required for recruiting E249. When provided as the only source of Uba2 in otherwise WT cells, all the Uba2 point mutants, including the Uba2C162S single mutant and the six Uba2 double point mutants, reduced SUMO conjugation (Fig. 5g) without impairing cell growth (Supplementary Fig. 10). Cells expressing Aos1E346V continued to accumulate conjugates, but the aos1-E346V uba2-C162S double mutant did not.

Taken together, our results suggest that long-term loss of Ulp2 SUMO protease activity favors countervailing partial loss-of-function mutations in genes encoding SUMO ligation pathway enzymes, particularly the essential Ubc9 (E2) and Uba2/Aos1 (E1) enzymes.

UBC9 and UBA2 mutations prevent aneuploidy in nascent ulp2Δ

To test the hypothesis that ulp2Δ aneuploidy could be directly suppressed by these balancing mutations in SUMO-ligating enzymes, we measured chromosome copy number, as well as cell growth, cell-cycle progression, and SUMO conjugates, in nascent ulp2Δ cells that carried ubc9, uba2, or aos1 missense mutations (Fig. 6a). Ubc9K27N expression efficiently suppressed the development of aneuploidy and the other mutant traits in low-passage ulp2Δ cells (Fig. 6b–e). Notably, even though provision of the single point mutant Uba2C162S did not suppress the growth and cell-cycle defects of nascent ulp2Δ cells, it slightly reduced levels of HMW SUMO-conjugated proteins and prevented the development of ChrXII (but not ChrI) disomy (Fig. 6f–i). Aneuploidy and the other defects of cells newly depleted of Ulp2 were also prevented by all tested uba2 double point mutants and the uba2C162S aos1E346V double mutant (Fig. 6f–m). These suppression results with nascent ulp2 null cells strongly support the contention that the E1 and E2 missense mutations isolated through long-term adaptation to Ulp2 loss are directly responsible for the recovery from aneuploidy and the suppression of the growth and stress resistance defects.

Fig. 6

Mutations in Ubc9, Uba2, and Aos1 suppress ulp2Δ aneuploidy and other defects. a Plasmid eviction strategy to test ubc9, uba2, and uba2 aos1 mutants that were also ulp2Δ. b, f, j Growth assays of the indicated strains. After spotting cells in fivefold serial dilutions, SD–Leu plates were incubated for 2 days at 30 °C. c, g, k Flow cytometry analysis of DNA content of the indicated strains. d, h, l Immunoblot analysis of SUMO conjugates in whole-cell lysates. e, i, m qPCR ploidy assays. Error bars indicate the SD calculated from two independent experiments


Following an acute loss of the Ulp2 SUMO protease, yeast respond by developing a specific two-chromosome aneuploidy18. While this rapid adaptive response helps stave off inviability, the mutant has many severe defects. The present study demonstrates that upon extended laboratory evolution, the extra chromosomes are lost in step-wise fashion. Remarkably, despite the complete absence of Ulp2, these evolved euploid cells acquire nearly normal growth and cell-cycle characteristics. Homeostasis appears to be restored in most cases by a combination of two mechanisms (Fig. 7). First, partial loss-of-function mutations to the essential E1 or E2 SUMO pathway enzymes reduce the excess accumulation of polySUMO-modified proteins caused by loss of Ulp2. Second, regulation of ribosome biogenesis, which is tightly controlled by the SUMO system, is altered such that overexpression of RP genes is reversed and snoRNAs are broadly upregulated, the latter likely through attenuated Ccr4-dependent transcriptional control. These data demonstrate a striking flexibility of cells in their response to loss of an essential gene: a specific but transient aneuploid state followed by distinct evolutionary trajectories capable of resolving the chromosome imbalances and restoring normal growth and stress resistance. Such interdependent adaptive mechanisms likely have relevance to other long-term cellular stress responses, including the evolution of tumor cells and aging.

Fig. 7

Short-term and long-term adaptive mechanisms caused by loss of Ulp2. Proposed model showing that yeast have short-term and long-term adaptive mechanisms that allow survival of a dysregulated SUMO system caused by loss of Ulp2. Loss of Ulp2 leads to accumulation of polySUMO-conjugated substrates, enhanced expression of genes encoding ribosomal proteins and reduced cell fitness (irregular cell outline). Duplication of ChrI and ChrXII provides a transient adaptive solution to amplify three protein-coding genes, CCR4, CLN3, and CCW12, and several snoRNA genes, SNR61, SNR55, and SNR57. Following evolution over many cell generations, disomies of both ChrI and XII are eliminated, concomitant with mutations in UBC9, UBA2, or AOS1. These SUMO-ligating enzyme mutations reduce SUMO conjugation and suppress the growth defects of ulp2Δ cells. Upregulation of numerous snoRNA genes appears to promote ribosome biogenesis, which is normally tightly regulated by the SUMO system

Yona et al.7 previously found that disomies induced by culturing yeast at either high temperature or high pH were eventually resolved even in the continued presence of the stress. Resolution of aneuploidy following the loss of an essential gene has not be reported previously to our knowledge. Our data indicate that different aneuploid ulp2Δ lines undergo variable but to some extent predictable adaptive evolutionary changes to compensate for the missing gene in ways that allows normal chromosome numbers to be restored. Predictable evolutionary trajectories were previously observed in yeast strains in response to the removal of an important cell polarity factor, although this did not involve an initial aneuploid state50.

The different genetic alterations of separately evolved aneuploid ulp2Δ lines is in some ways reminiscent of the genetic heterogeneity that characterizes human tumors51. Over 90% of solid tumors are aneuploid, but extensive intratumor variability is observed. In some tumors, distinct mutations affecting the same tumor driver genes were found, suggesting convergent evolution leading to neoplastic growth and metastasis. In the transiently aneuploid ulp2Δ lines in our study, missense mutations in three different SUMO-conjugation factors were identified, and for Uba2, multiple independent missense mutations, as these cells evolved back to a fast-growing euploid state.

A natural experiment in the loss of the ULP2 gene might have occurred in microsporidial species. Microsporidia are intracellular parasites related to fungi that have undergone drastic genome reductions52. In Encephalitozoon spp., which have only ~2000 genes, no clear ULP2 ortholog is found, although at least a rudimentary SUMO ligation system still appears to exist based on available genome sequences. Different microsporidial species might have independently evolved ways of maintaining a balance between SUMO conjugation and deconjugation as components of the SUMO system were lost or reduced.

It should be possible in many cases to trace the complex pathways of long-term genetic change occurring in response to loss or inhibition of cellular enzymes, as demonstrated in the current study. The ability of aneuploidy to serve as a suboptimal but rapid response to cellular stress, is now well documented; However, long-term responses to aneuploidy have been only minimally investigated7. These responses may not only be relevant to tumorigenesis, as noted above, but to aging and drug resistance. For example, we found that yeast ulp2 mutants are unusually resistant to rapamycin. Rapamycin treatment boosts longevity in many species, and mTORC1 inhibitors are now being considered for use in humans53. Our data suggest that genetic background and tissue heterogeneity may have major effects on the efficacy of such treatments.


Yeast strains

Yeast strains used in this study are listed in Supplementary Table 1. Standard techniques were used for strain construction. The mutant ulp2Δ ubc9 strain was made by replacing the WT UBC9 ORF in MHY1328 (ulp2Δ/ULP2 diploid) with a TRP1 marker; the resulting strain was transformed with YCplac33-UBC9, sporulated and dissected, and the doubly deleted haploid was isolated. After transforming in the pRS315-ubc9 plasmid, YCplac33-UBC9 was evicted by two consecutive streakings on 5-FOA. The ulp2Δ uba2 and ulp2Δ uba2 aos1 strains were made in analogous fashion except the UBA2 gene was replaced by a kanMX6 module and AOS1 by a natMX4 cassette. To generate MHY9393, MHY10229 and MH10230 strains, the C-terminal insertion cassettes of CCR4–6xGly-3xFlag, NOT5–6xGly-3xFlag and RAP1–6xGly-3xFlag were constructed by PCR amplification from pFA6a-6xGly-3xFlag::KanMX654 and transformed into MHY1379 cells (ulp2Δ + YCplac33-ULP2 haploid).

To create yeast strains newly null for ULP2, MHY1379 cells with or without a LEU2-marked plasmid carrying a gene(s) of interest were streaked on 5-FOA or 5-FOA–Leu plates twice in succession to evict the ULP2 cover plasmid. All strains were verified by PCR and/or immunoblot analysis.

Yeast growth conditions

Cells were grown at 30 °C in YPD or synthetic defined (SD) minimal medium with the appropriate supplements. For growth analysis on plates, cultures in exponential growth were normalized to an A600 of 0.1, which were subject to fivefold serial dilutions. Dilution series were spotted onto appropriate media, and the plates were incubated at 30  or 37 °C for 2–5 days. To induce Ulp2 degradation via the AID* tag and ULP2 mRNA turnover via the neomycin-inducible hammerhead ribozyme (HHR) in the 3′ UTR of ULP2, cells were incubated in YPD with 500 μM indole-3-acetic acid (IAA) and 100 μg/ml of neomycin55,56 and then diluted daily 1:120 into fresh medium containing the drugs for 16 days. For laboratory evolution experiments, cells were grown to stationary phase in YPD and then diluted 1:120 into fresh YPD medium, as described previously7. This process was repeated daily (6.9 generations per day).


Plasmids used in this study are listed in Supplementary Table 2. To create high-copy plasmids with ChrXII subfragments from the 11-b5, 11-c5, 11-e11, or 11-f11 genomic library clones, the ORFs with 0.6–1 kb of sequence upstream and downstream of the ORF were PCR-amplified from the genomic library plasmids and cloned into the pGP564 plasmid. Exceptions to this were the following: For pGP564-REX3 + SNR6 + YLR108C, pGP564-YLR334C + tE(UUC)L + NUP2 or pGP564-SGD1, a 5-kb SacI fragment from 11-b5, 4.5-kb PstI fragment from 11-e11, and 5.5-kb SacI fragment from 11-f11, respectively, were inserted into pGP564. pGP564-REC102 was generated by religation of the 11-e11 vector fragment containing the REC102 ORF after PstI digestion. For the ubc9 and uba2 plasmids, the mutated ORF with ~0.8-kb of upstream and downstream sequences were amplified by PCR and cloned into pRS315. The amplified ORFs of AOS1 or aos1E346V with ~0.8-kb of flanking sequences were cloned into pRS315-UBA2, pRS315-uba2C162S or YCplac33-UBA2. For overexpression of HIS-SMT3, the allele was amplified by PCR from MHY5339 and then cloned into p425-GPD. All constructs were confirmed by DNA sequencing.

RNA isolation and RNA-seq analysis

Total RNA was extracted as previously described18. Briefly, one OD600 equivalent of cells grown to mid-exponential phase was used for RNA isolation using the RNeasy kit (Qiagen). The Ambion DNA-free DNA removal kit was used to remove DNA contaminants.

Twelve strand-specific sequencing libraries, three replicates per condition, were produced from the purified total RNA samples by the Illumina TruSeq stranded protocol. The libraries underwent 76-bp paired-end sequencing using an Illumina HiSeq 2500 according to Illumina protocols, generating an average of 14 million paired-end reads per library. For each read, we trimmed the first six nucleotides and the last nucleotides at the point where the Phred score of an examined base fell below 20 using in-house scripts. If, after trimming, the read was shorter than 45 bp, the entire read was discarded. Trimmed reads were mapped to the S. cerevisiae genome (Ensembl R64–1–1) with Tophat v2.1.157 using the very-sensitive preset, first-strand library type, and providing the corresponding gene model annotation. Only the reads that mapped to a single unique location within the genome, with a maximum of two mismatches in the anchor region of the spliced alignment, were reported in these results. We used the default settings for all other Tophat options. Tophat alignments were then processed by Cuffdiff (Cufflinks v2.2.158) to obtain differential gene expression using first-strand library type, providing gene model annotation, and the genome sequence file for detection and correction of sequence-specific bias that random hexamer can cause during library preparation.

Reverse transcription-polymerase chain reactions (RT-PCRs)

One microgram of RNA was used in reverse transcription reactions using the iScript cDNA synthesis kit (Bio-Rad). The oligonucleotide sequences used for qPCR are listed in Supplementary Table 3. Diluted cDNA (1:200) was used in qPCR reactions to determine the expression of ribosomal protein genes RPL12B and RPS18B, snoRNA genes SNR30 and SNR60, and the ACT1 or SPT15 controls. To measure expression of rRNA 18s and 25s, cDNA was diluted to 1:1,000. Each qPCR reaction was performed in technical triplicate. Relative RNA levels were calculated using the comparative Ct method (ΔΔCt)59.

DNA-sequencing (seq) analysis

Genomic DNA was extracted from 1 OD600 equivalent of cells using a standard phenol/chloroform extraction method. Whole-genome sequencing was then performed by the Yale Center for Genome Analysis, using 2 × 100 bp sequencing on Illumina HiSeq 2500 instruments, to an average depth of 500x per sample. The reads were aligned to the S. cerevisiae genome using BWA MEM v0.7.15, and a joint calling of variants was performed using freebayes v0.9.14 with options (-P 0.5 -E 0 -q 10 -C 5).

qPCR ploidy assay

Chromosome copy number was determined by qPCR ploidy assays according to the protocol of Pavelka et al.60 as described previously18. Briefly, DNA samples were prepared by the method described above. The oligonucleotide sequences used for qPCR are listed in Supplementary Table 3. Triplicate qPCR reactions were performed using the iQ SYBR Green Supermix kit in a Roche LightCycler 480 instrument, and the qPCR results were analyzed by the modified Ct method59. Ct values for each chromosome were normalized to the median Ct value for each cell, and then ∆Ct was represented as relative ratio to WT control. For screening assays in Supplementary Fig. 6, each reaction was performed in technical duplicate.

Chromatin immunoprecipitation (ChIP)

ChIP experiments were done using established protocols18,61. Briefly, cells grown to mid-log phase in 200 ml of SD medium with suitable supplements were cross-linked with formaldehyde for 20 min and quenched with glycine. Cell pellets were lysed with glass beads and then sonicated to produce DNA fragments of ~500 bp. TAP-tagged, Flag-tagged and His-tagged proteins in clarified extracts were precipitated with 20 µl of IgG-Sepharose beads (17-0969-01, GE Healthcare), anti-Flag agarose beads (A2220, Sigma) and Ni-NTA agarose beads (R90115, Thermo Scientific), respectively. Following washings, eluted chromatin fragments were treated with pronase (Roche), and DNA was purified by phenol/chloroform extraction. The oligonucleotide sequences used for ChIP qPCR are listed in Supplementary Table 3. qPCR assays were performed using diluted template DNA (1:8 dilution for IP DNA and 1:1000 dilution for input DNA), and signals were normalized to the internal control (a fragment amplified from an untranscribed region on ChrIV) and input DNA.


Preparation of yeast whole-cell extracts and immunoblotting were carried out as described previously62. Levels of the Ulp2-AID-6Flag fusion protein, SUMO conjugate profiles, and Pgk1 were analyzed by immunoblotting with 1:2000 dilutions of anti-Flag (F3165, Sigma), anti-SUMO63 and anti-Pgk1 (459250, Molecular Probes) antibodies, respectively. Sumoylated Rap1 was detected according to previous reports with little modification36. Specifically, TCA-extracted proteins from 50 OD600 of cells were resuspended in 0.6 ml of sodium dodecyl sulphate (SDS)-sample buffer with 50 µl of unbuffered 2 M Tris, and then heated to 100 °C for 10 min. After centrifugation, 0.4 ml of supernatants were diluted with 0.8 ml of buffer (50 mM Tris HCl [pH 7.4], 5 mM EDTA, 150 mM NaCl, 1% Triton-X100) containing 20 mM NEM, immunoprecipitated with anti-Flag agarose beads (A2220, Sigma) for 4 h at 4 °C and then finally eluted into SDS-sample buffer by boiling for 5 min. Both IP and INPUT samples were analyzed by sodium dodecyl sulphate-polyacrylamide gel electrophoresis (SDS-PAGE) and immunoblotting as described above. For analysis of ribosomal proteins, TCA-extracted proteins were separated by Tricine-SDS-PAGE and then detected by immunoblotting using 1:1000 of anti-Rpl32 antibody (PA5–69070, Invitrogen). Uncropped blots are presented in a Supplementary Fig. 11.

Flow cytometry analysis

Yeast DNA content was analyzed by flow cytometry as previously described18,64. Cells in exponential growth were fixed in 70% ethanol, digested with RNase A, and then stained with propidium iodide at 50 μg/ml final concentration. The analysis was carried out using a FACS LSRII flow cytometer (BD Biosciences) with a green laser (150 mW at 532 nm). Data were analyzed using FlowJo ver. 8 (Tree Star) and illustrated with two peaks indicating DNA contents, 1 C (unreplicated DNA) and 2 C (replicated DNA).

Construction of ULP2-AID*-6FLAG-neo-HHR-B2

Directly after the stop codon in the gene for the Ulp2-AID*-6FLAG fusion protein65 is a 21-bp linker, the neo-HHR-B2 sequence (91 bp), a 19-bp A-rich linker56 and the authentic ULP2 3′UTR sequence. Marker-free genome editing was achieved by CRISPR/Cas9-mediated cleavage within the original ULP2 stop codon (TAG) and insertion of a 545-bp insert with the aforementioned allele. Specifically, a PCR fragment including the 545 bp AID*-6FLAG-neo-HHR-B2 cassette plus a 5′ flanking region from ULP2 ORF nucleotides 3058–3102 and a 3′ flanking region from ULP2 3′UTR nucleotides 1–45 was amplified from plasmid pHyg-AIDstar-6FLAG_neo_HHR_B2 and used for integration. The pHyg-AIDstar-6FLAG_neo_HHR_B2 plasmid was generated by inserting the neo_HHR_B2 sequence amplified from plasmid pBT3-K2–3’fRzSu-AG-lib4-B265 (kind gift of J. Hartig, U. Konstanz) into XbaI/BglII-cut pHyg-AIDstar-6FLAG56.

A one-vector system with sgRNA and Cas9 expression cassettes in a single plasmid66 was used to direct genomic integration. A duplex of STK#58 (GATCT-ATGCGTGCGAGTGCTTTCAGTTTTAGAGCTAG) and STK#59 CTAGCTCTAAAACT-GAAAGCACTCGCACGCATA) oligonucleotides was cloned into SwaI,Bcl-cut pML104;66 the resulting pML104-gRNA-ULP2CT plasmid encodes the sgRNA that directs ULP2 cleavage. The 635 bp PCR fragment and pML104-gRNA-ULP2CT were co-transformed into Y884 yeast. The desired insert was confirmed by PCR and DNA sequencing. The URA3-marked pML104-gRNA-ULP2CT plasmid was then evicted on a 5-FOA, resulting in yeast strain Y911. Y884 was created by integrating MscI-linearized pRS303-ADH1-AFB2 (kind gift of Helle Ulrich, IMB Mainz) at the his3Δ1 locus of strain BY4741. The strain expresses the A. thaliana F-box protein AFB2 from the yeast ADH1 promoter.

Data availability

The RNA-seq and DNA-seq data used in this publication have been deposited in Gene Expression Omnibus (GEO) with accession GSE121898 and GSE121899, respectively. A reporting summary for this Article is available as a Supplementary Information file. All other data supporting the findings of this study are available from the corresponding authors on reasonable request.


  1. 1.

    Germain, R. N. The art of the probable: system control in the adaptive immune system. Science 293, 240–245 (2001).

    CAS  PubMed  Article  Google Scholar 

  2. 2.

    Kyrou, I. & Tsigos, C. Stress hormones: physiological stress and regulation of metabolism. Curr. Opin. Pharmacol. 9, 787–793 (2009).

    CAS  PubMed  Article  Google Scholar 

  3. 3.

    Mulla, W., Zhu, J. & Li, R. Yeast: a simple model system to study complex phenomena of aneuploidy. FEMS Microbiol. Rev. 38, 201–212 (2014).

    CAS  PubMed  Article  Google Scholar 

  4. 4.

    Rosenberg, S. M. Evolving responsively: adaptive mutation. Nat. Rev. Genet. 2, 504–515 (2001).

    CAS  PubMed  Article  Google Scholar 

  5. 5.

    Kronholm, I. & Collins, S. Epigenetic mutations can both help and hinder adaptive evolution. Mol. Ecol. 25, 1856–1868 (2016).

    CAS  PubMed  Article  Google Scholar 

  6. 6.

    Galluzzi, L., Pedro, J. M. B. S., Kepp, O. & Kroemer, G. Regulated cell death and adaptive stress responses. Cell. Mol. Life Sci. 73, 2405–2410 (2016).

    CAS  PubMed  Article  Google Scholar 

  7. 7.

    Yona, A. H. et al. Chromosomal duplication is a transient evolutionary solution to stress. Proc. Natl Acad. Sci. USA 109, 21010–21015 (2012).

    ADS  CAS  PubMed  Article  Google Scholar 

  8. 8.

    Gordon, D. J., Resio, B. & Pellman, D. Causes and consequences of aneuploidy in cancer. Nat. Rev. Genet. 13, 189–203 (2012).

    CAS  PubMed  Article  Google Scholar 

  9. 9.

    Dragosits, M. & Mattanovich, D. Adaptive laboratory evolution—principles and applications for biotechnology. Microb. Cell Fact 12, 64 (2013).

  10. 10.

    Nishant, K. T., et al. The baker’s yeast diploid genome is remarkably stable in vegetative growth and meiosis. PLoS Genet. 6, e1001109 (2010).

  11. 11.

    Lynch, M. et al. A genome-wide view of the spectrum of spontaneous mutations in yeast. Proc. Natl Acad. Sci. USA 105, 9272–9277 (2008).

    ADS  CAS  PubMed  Article  Google Scholar 

  12. 12.

    Zhu, Y. O., Siegal, M. L., Hall, D. W. & Petrov, D. A. Precise estimates of mutation rate and spectrum in yeast. Proc. Natl Acad. Sci. USA 111, E2310–E2318 (2014).

    ADS  CAS  PubMed  Article  Google Scholar 

  13. 13.

    Marsit, S. et al. Evolutionary biology through the lens of budding yeast comparative genomics. Nat. Rev. Genet. 18, 581–598 (2017).

    CAS  PubMed  Article  Google Scholar 

  14. 14.

    Roth, J. R., Kugelberg, E., Reams, A. B., Kofoid, E. & Andersson, D. I. Origin of mutations under selection: The adaptive mutation controversy. Annu. Rev. Microbiol. 60, 477–501 (2006).

    CAS  PubMed  Article  Google Scholar 

  15. 15.

    Flotho, A. & Melchior, F. Sumoylation: A regulatory protein modification in health and disease. Annu. Rev. Biochem. 82, 357–385 (2013).

    CAS  PubMed  Article  Google Scholar 

  16. 16.

    Hickey, C. M., Wilson, N. R. & Hochstrasser, M. Function and regulation of SUMO proteases. Nat. Rev. Mol. Cell Bio. 13, 755–766 (2012).

    CAS  Article  Google Scholar 

  17. 17.

    Li, S. J. & Hochstrasser, M. The yeast ULP2 (SMT4) gene encodes a novel protease specific for the ubiquitin-like Smt3 protein. Mol. Cell. Biol. 20, 2367–2377 (2000).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  18. 18.

    Ryu, H. Y., Wilson, N. R., Mehta, S., Hwang, S. S. & Hochstrasser, M. Loss of the SUMO protease Ulp2 triggers a specific multichromosome aneuploidy. Genes Dev. 30, 1881–1894 (2016).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  19. 19.

    Ryu, H. Y. & Hochstrasser, M. Adaptive aneuploidy counters a dysregulated SUMO system. Cell Cycle 16, 383–385 (2017).

    CAS  PubMed  Article  Google Scholar 

  20. 20.

    Panse, V. G. et al. Formation and nuclear export of preribosomes are functionally linked to the small-ubiquitin-related modifier pathway. Traffic 7, 1311–1321 (2006).

    CAS  PubMed  Article  Google Scholar 

  21. 21.

    Venema, J. & Tollervey, D. Ribosome synthesis in Saccharomyces cerevisiae. Annu. Rev. Genet. 33, 261–311 (1999).

    CAS  PubMed  Article  Google Scholar 

  22. 22.

    Tollervey, D. & Kiss, T. Function and synthesis of small nucleolar RNAs. Curr. Opin. Cell Biol. 9, 337–342 (1997).

    CAS  PubMed  Article  Google Scholar 

  23. 23.

    Westman, B. J. et al. A proteomic screen for nucleolar SUMO targets shows SUMOylation modulates the function of Nop5/Nop58. Mol. Cell 39, 618–631 (2010).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  24. 24.

    Schwienhorst, I., Johnson, E. S. & Dohmen, R. J. SUMO conjugation and deconjugation. Mol. General. Genet. 263, 771–786 (2000).

    CAS  Article  Google Scholar 

  25. 25.

    Sheltzer, J. M. & Amon, A. The aneuploidy paradox: costs and benefits of an incorrect karyotype. Trends Genet. 27, 446–453 (2011).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  26. 26.

    Santaguida, S. & Amon, A. Short- and long-term effects of chromosome mis-segregation and aneuploidy. Nat. Rev. Mol. Cell Bio. 16, 473–485 (2015).

    CAS  Article  Google Scholar 

  27. 27.

    Pavelka, N., Rancati, G. & Li, R. Dr Jekyll and Mr Hyde: role of aneuploidy in cellular adaptation and cancer. Curr. Opin. Cell Biol. 22, 809–815 (2010).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  28. 28.

    Chymkowitch, P. et al. Sumoylation of Rap1 mediates the recruitment of TFIID to promote transcription of ribosomal protein genes. Genome Res. 25, 897–906 (2015).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  29. 29.

    Finkbeiner, E., Haindl, M., Raman, N. & Muller, S. SUMO routes ribosome maturation. Nucleus 2, 527–532 (2011).

    PubMed  Article  Google Scholar 

  30. 30.

    Maxwell, E. S. & Fournier, M. J. The small nucleolar RNAs. Annu. Rev. Biochem. 64, 897–934 (1995).

    CAS  PubMed  Article  Google Scholar 

  31. 31.

    Williams, G. T. & Farzaneh, F. Are snoRNAs and snoRNA host genes new players in cancer? Nat. Rev. Cancer 12, 84–88 (2012).

    CAS  PubMed  Article  Google Scholar 

  32. 32.

    Bachellerie, J. P., Cavaille, J. & Huttenhofer, A. The expanding snoRNA world. Biochimie 84, 775–790 (2002).

    CAS  PubMed  Article  Google Scholar 

  33. 33.

    Michel, C. I. et al. Small nucleolar RNAs U32a, U33, and U35a are critical mediators of metabolic stress. Cell Metab. 14, 33–44 (2011).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  34. 34.

    Youssef, O. A. et al. Potential role for snoRNAs in PKR activation during metabolic stress. Proc. Natl Acad. Sci. USA 112, 5023–5028 (2015).

    ADS  CAS  PubMed  Article  Google Scholar 

  35. 35.

    Chu, L. et al. Multiple myeloma-associated chromosomal translocation activates orphan snoRNA ACA11 to suppress oxidative stress. J. Clin. Invest. 122, 2793–2806 (2012).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  36. 36.

    Gillies, J. et al. SUMO pathway modulation of regulatory protein binding at the ribosomal DNA locus in Saccharomyces cerevisiae. Genetics 202, 1377-+ (2016).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  37. 37.

    Liang, J. et al. Recruitment of a SUMO isopeptidase to rDNA stabilizes silencing complexes by opposing SUMO targeted ubiquitin ligase activity. Genes Dev. 31, 802–815 (2017).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  38. 38.

    Laribee, R. N., Hosni-Ahmed, A., Workman, J. J. & Chen, H. Ccr4-not regulates RNA polymerase I transcription and couples nutrient signaling to the control of ribosomal RNA biogenesis. PLoS Genet. 11, e1005113 (2015).

    PubMed  PubMed Central  Article  Google Scholar 

  39. 39.

    Azzouz, N., Panasenko, O. O., Colau, G. & Collart, M. A. The CCR4-NOT complex physically and functionally interacts with TRAMP and the nuclear exosome. PLoS ONE. 4, e6760 (2009).

    ADS  PubMed  PubMed Central  Article  Google Scholar 

  40. 40.

    Azzouz, N. et al. Specific roles for the Ccr4-Not complex subunits in expression of the genome. RNA 15, 377–383 (2009).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  41. 41.

    Jones, G. M. et al. A systematic library for comprehensive overexpression screens in Saccharomyces cerevisiae. Nat. Methods 5, 239–241 (2008).

    CAS  PubMed  Article  Google Scholar 

  42. 42.

    Ragni, E. et al. The genetic interaction network of CCW12, a Saccharomyces cerevisiae gene required for cell wall integrity during budding and formation of mating projections. BMC Genom. 12, 107 (2011).

    CAS  Article  Google Scholar 

  43. 43.

    Mrsa, V. et al. Deletion of new covalently linked cell wall glycoproteins alters the electrophoretic mobility of phosphorylated wall components of Saccharomyces cerevisiae. J. Bacteriol. 181, 3076–3086 (1999).

    CAS  PubMed  PubMed Central  Google Scholar 

  44. 44.

    Christiano, R., Nagaraj, N., Frohlich, F. & Walther, T. C. Global proteome turnover analyses of the Yeasts S. cerevisiae and S. pombe. Cell Rep. 9, 1959–1965 (2014).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  45. 45.

    Hardwick, K. C., Johnston, R. C., Smith, D. L. & Murray, A. W. MAD3 encodes a novel component of the spindle checkpoint which interacts with Bub3p, Cdc20p, and Mad2p. J. Cell Biol. 148, 871–882 (2000).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  46. 46.

    Tevzadze, G. G., Pierce, J. V. & Esposito, R. E. Genetic evidence for a SPO1-dependent signaling pathway controlling meiotic progression in yeast. Genetics 175, 1213–1227 (2007).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  47. 47.

    Schwartz, D. C., Felberbaum, R. & Hochstrasser, M. The ulp2 SUMO protease is required for cell division following termination of the DNA damage checkpoint. Mol. Cell. Biol. 27, 6948–6961 (2007).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  48. 48.

    Pichler, A., Fatouros, C., Lee, H. & Eisenhardt, N. SUMO conjugation—a mechanistic view. Biomol. Concepts 8, 13–36 (2017).

    CAS  PubMed  Article  Google Scholar 

  49. 49.

    Lois, L. M. & Lima, C. D. Structures of the SUMO E1 provide mechanistic insights into SUMO activation and E2 recruitment to E1. EMBO J. 24, 439–451 (2005).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  50. 50.

    Laan, L., Koschwanez, J. H. & Murray, A. W. Evolutionary adaptation after crippling cell polarization follows reproducible trajectories. Elife 4, pii: e09638 (2015).

  51. 51.

    Gerlinger, M. et al. Intratumor heterogeneity and branched evolution revealed by multiregion sequencing. N. Engl. J. Med. 366, 883–892 (2012).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  52. 52.

    Haag, K. L. et al. Evolution of a morphological novelty occurred before genome compaction in a lineage of extreme parasites. Proc. Natl Acad. Sci. USA 111, 15480–15485 (2014).

    ADS  CAS  PubMed  Article  Google Scholar 

  53. 53.

    Lamming, D. W., Ye, L., Sabatini, D. M. & Baur, J. A. Rapalogs and mTOR inhibitors as anti-aging therapeutics. J. Clin. Invest. 123, 980–989 (2013).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  54. 54.

    Funakoshi, M. & Hochstrasser, M. Small epitope-linker modules for PCR-based C-terminal tagging in Saccharomyces cerevisiae. Yeast 26, 185–192 (2009).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  55. 55.

    Nishimura, K., Fukagawa, T., Takisawa, H., Kakimoto, T. & Kanemaki, M. An auxin-based degron system for the rapid depletion of proteins in nonplant cells. Nat. Methods 6, 917–U978 (2009).

    CAS  PubMed  Article  Google Scholar 

  56. 56.

    Klauser, B., Rehm, C., Summerer, D. & Hartig, J. S. Engineering of ribozyme-based aminoglycoside switches of gene expression by in vivo genetic selection in Saccharomyces cerevisiae. Method. Enzymol. 550, 301–320 (2015).

    CAS  Article  Google Scholar 

  57. 57.

    Trapnell, C., Pachter, L. & Salzberg, S. L. TopHat: discovering splice junctions with RNA-Seq. Bioinformatics 25, 1105–1111 (2009).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  58. 58.

    Trapnell, C. et al. Transcript assembly and quantification by RNA-Seq reveals unannotated transcripts and isoform switching during cell differentiation. Nat. Biotechnol. 28, 511–515 (2010).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  59. 59.

    Schmittgen, T. D. & Livak, K. J. Analyzing real-time PCR data by the comparative C(T) method. Nat. Protoc. 3, 1101–1108 (2008).

    CAS  PubMed  Article  Google Scholar 

  60. 60.

    Pavelka, N. et al. Aneuploidy confers quantitative proteome changes and phenotypic variation in budding yeast. Nature 468, 321–325 (2010).

    ADS  CAS  PubMed  PubMed Central  Article  Google Scholar 

  61. 61.

    Ryu, H.-Y. & Ahn, S. H. Yeast histone H3 lysine 4 demethylase Jhd2 regulates mitotic rDNA condensation. BMC Biol. 12, 75 (2014).

    PubMed  PubMed Central  Article  Google Scholar 

  62. 62.

    Kroetz, M. B., Su, D. & Hochstrasser, M. Essential role of nuclear localization for Yeast Ulp2 SUMO protease function. Mol. Biol. Cell 20, 2196–2206 (2009).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  63. 63.

    Li, S. J. & Hochstrasser, M. A new protease required for cell-cycle progression in yeast. Nature 398, 246–251 (1999).

    ADS  CAS  PubMed  Article  Google Scholar 

  64. 64.

    Haase, S. B. & Lew, D. J. Flow cytometric analysis of DNA content in budding yeast. Methods Enzymol. 283, 322–332 (1997).

    CAS  PubMed  Article  Google Scholar 

  65. 65.

    Morawska, M. & Ulrich, H. D. An expanded tool kit for the auxin-inducible degron system in budding yeast. Yeast 30, 341–351 (2013).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  66. 66.

    Laughery, M. F. et al. New vectors for simple and streamlined CRISPR-Cas9 genome editing in Saccharomyces cerevisiae. Yeast 32, 711–720 (2015).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

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We thank Christopher Hickey for comments on the manuscript. This work was supported by NIH grant R01 GM053756 to M.H.

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H.Y.R. contributed to the experimental design, performed most of experiments and drafted the manuscript. F.L.G. and J.K. analyzed the RNA-seq and DNA-seq data, respectively. S.S.H. carried out flow cytometry analysis. C.R. and S.G.K. made the strain used for the Ulp2-AID* depletion analysis. M.H. designed the study, analyzed the data, and wrote the final version of the manuscript.

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Correspondence to Mark Hochstrasser.

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Ryu, HY., López-Giráldez, F., Knight, J. et al. Distinct adaptive mechanisms drive recovery from aneuploidy caused by loss of the Ulp2 SUMO protease. Nat Commun 9, 5417 (2018).

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