The Histone H2B Arg95 residue links the Pheromone Response Pathway to Rapamycin-Induced G1 Arrest in Yeast

doi:10.21203/rs.3.rs-1439695/v1

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The Histone H2B Arg95 residue links the Pheromone Response Pathway to Rapamycin-Induced G1 Arrest in Yeast

https://doi.org/10.21203/rs.3.rs-1439695/v1

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published 14 Jun, 2022

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Rapamycin is an immunosuppressant used for treating many types of diseases such as kidney carcinomas. In yeast, rapamycin inhibits the TORC1 kinase signaling pathway causing rapid alteration in gene expression and ultimately cell cycle arrest in G 1 through mechanisms that are not fully understood. Herein, we screened a histone mutant collection and report that one of the mutants, H2B R95A, is strikingly resistant to rapamycin due to a defective cell cycle arrest. We show that the H2B R95A causes defects in the expression of a subset of genes of the pheromone pathway required for α factor-induced G 1 arrest. The expression of the STE5 gene and its encoded scaffold protein Ste5, required for the sequential activation of the MAPKs of the pheromone pathway, is greatly reduced in the H2B R95A mutant. Similar to the H2B R95A mutant, cells devoid of Ste5 are also resistant to rapamycin. Rapamycin-induced G 1 arrest does not involve detectable phosphorylation of the MAPKs, Kss1 and Fus3, as reported for α factor-induced G 1 arrest. However, we observed a sharp induction of the G 1 cyclin Cln2 (~ 3- to 4-fold) in the ste5Δ mutant within 30 mins of exposure to rapamycin. Our data provide a new insight whereby rapamycin signaling via the Torc1 kinase may exploit the pheromone pathway to arrest cells in the G 1 phase.

histone H2B

transcription

MAP kinases and pheromone response

rapamycin

cyclin Cln2

Torc1 kinase

Rapamycin is an immunosuppressant used for treating diseases such as kidney carcinomas [1-3]. In Saccharomyces cerevisiae, rapamycin binds to the peptidyl-prolyl isomerase Fpr1 leading to the inhibition of the Target of Rapamycin (TOR) kinase that forms the TOR Complex 1 (Torc1) [4, 5]. Torc1 consists of either the Tor1 or the Tor2 kinase, a putative scaffold protein Kog1, Lst8, and Tco89 [4, 5]. Torc1 controls growth in response to nutrients by regulating translation, transcription, ribosome biogenesis, nutrient transport, autophagy, and cell cycle [4, 6-8]. The inhibition of Torc1 by rapamycin mimics nutrient starvation and causes an array of physiological changes that include global changes in gene expression, phosphorylation/dephosphorylation of various factors, decreased cell growth, degradation of proteins, and ultimately cell cycle arrest in the G₁ phase [4, 9-11]. The exact molecular mechanism that leads to G₁ arrest following rapamycin treatment in yeast is a complex process that has not been fully delineated, although it is believed to be indirectly derived from a combination of events that include (i) inhibition of protein synthesis due to the degradation of the protein translational initiation factors eIF4G1 and eIF4G2 [10, 12-14], (ii) reduced expression of genes encoding ribosomal proteins [8], (iii) the subsequent transcriptional downregulation of the cyclin genes involved in the transition of cells from the G₁ to the S phase [10], (vi) the specific phosphorylation at the C-terminal domain of RNA polymerase II[15], and (v) the phosphorylation and stabilization of the Sic1 inhibitor protein that inhibits the B-type cyclin-dependent protein kinase [16-18].

We have previously shown that the peptidyl-prolyl isomerase Rrd1 is required to mediate cellular response to rapamycin by altering gene expression [6, 7, 19, 20]. Rrd1 is tightly bound to chromatin and interacts with RNA polymerase II (RNAPII) [6, 20]. It can isomerize the C-terminal domain of the large subunit of RNAPII and this may promote the redistribution of the polymerase along the genome in response to rapamycin [6, 20, 21]. Rrd1 has been shown to stimulate the association of RNAPII with the coding region of inducible genes besides those activated by rapamycin, but not with constitutively expressed genes [6, 21]. This Rrd1-dependent recruitment of RNAPII is associated with nucleosomal disassembly and transcription activation [6, 20, 21]. From these combined studies, it seems logical that the global gene expression pattern that ensues upon exposure to rapamycin must be governed by changes at the level of the chromatin structure. Indeed, it has been shown that a histone mutant H3 K56A causes yeast cells to display sensitivity to rapamycin, however, this mutation also sensitizes cells to a variety of DNA damaging agents, suggesting that the H3 K56A mutation has a broader role rather than a specific function towards rapamycin stress [22, 23]. Here, we hypothesized that specific histone residue(s) might be involved in facilitating gene expression such that cells mount a response to rapamycin. We, therefore, searched a collection of 442 histone mutants [24] for ones that failed to respond to rapamycin in an attempt to identify molecular pathways critical for rapamycin response at the level of chromatin. We report the identification of nine histone mutants, eight of which showed varying resistance to rapamycin, as compared to the other mutants and the wild type (WT). Of these mutants, H2B R95A displayed striking resistance to rapamycin, which correlated with an inability to undergo cell cycle arrest. Further analysis revealed that the H2B R95A was significantly defective in the expression of at least 26 genes that belong to the pheromone response pathway that is required for α factor-induced G₁ arrest. This mutant weakly expressed the STE5 gene and its encoding scaffold protein Ste5, required for the sequential activation of the MAPKs of the pheromone pathway. Cells lacking Ste5 exhibited nearly the same level of resistance to rapamycin as the H2B R95A mutant, suggesting that the rapamycin-resistant phenotype of this mutant is restricted to the pheromone response pathway. We show that rapamycin-induced G₁ arrest is independent of the phosphorylation of the MAPKs, Kss1 and Fus3, required for α factor-induced G₁ arrest. However, we unexpectedly observed a sharp induction of the G₁ cyclin Cln2 in the ste5Δ mutant within 30 mins of exposure to rapamycin, as compared to the WT. We provide some insights into the possible roles of the induced Cln2 level in the ste5Δ mutant, which might serve to promote cell proliferation in the presence of rapamycin.

Yeast strains, growth media, plasmid, and drugs—The yeast WT strains and the isogenic histone mutants used in this work (Supplementary Table S1) were from the SHIMA library, kindly provided by Dr. Ali Shilatifard (Kansas, USA) [24]. All other strains used in this study (Supplementary Table S1) were the WT BY4741 and the indicated isogenic mutants derived from the nonessential haploid mutant (D.R. laboratory resource) and the TAP-tagged collections provided by Dr. Hugo Wurtele (Montreal, Canada). Epitope-tagging of strains at the endogenous gene locus was performed as previously described [25]. Cells were grown at 30 ^oC for 24 hrs in either Yeast Peptone Dextrose (YPD, FORMEDIUM CCM0105) or SD minimal media. The single-copy plasmid pSTE5-GFP carrying the entire STE5 gene under its promoter and tagged with GFP was kindly provided by Dr. Peter M. Pryciak (University of Massachusetts medical school, Worcester, MA, USA). All chemical reagents including rapamycin, methyl methanesulfonate, 4-nitroquinoline-1-oxide, and sodium arsenite were purchased from Sigma, St Louis, USA.

Spotting test—The strains were grown in YPD media at 30 ^oC for 24 hrs. The OD600_nm was adjusted to 1.0 and serial dilutions of 1:10, 1:50, 1:100, 1:500, and 1:1000 were prepared using 96-well plates [6]. Four microliters of each dilution were spotted onto YPD solid media without and with 2.0 ng/ml of rapamycin. The plates were incubated at 30 ^oC and photographed after 48 hours using (Image Lab Touch Software, BioRad).

RNA extraction and RT- PCR—Yeast cultures were grown overnight, then collected the following day by centrifugation at 3220 x g for 5 mins. The pellets were washed once with sterile water, then processed for RNA extraction using RiboPure^TM yeast RNA purification kit as per the manufacturer protocol (Qiagen). RNA concentration and purity were checked by Nanodrop 2000. cDNA was prepared from the total RNA (0.5 µg) using high-capacity cDNA reverse transcription kit according to the manufacturer protocol (Thermofisher Scientific). Samples were run on Quanti Studio 6 Flex qPCR machine using PowerUp SYBR Green Master Mix (Thermofisher Scientific), ACT1 gene was used as the control for quantification of STE5 gene expression, and the primers used were as follow: ACT1-F, 5ʹ-TGGGTATCCAAGCACATCAA, ACT1-R, 5ʹ-TGATAAACCCGCTGAA CACA, STE5-F, 5ʹ-CGTCCGGAGCAAACTCTATC, and STE5-R, 5ʹ-ATGACCTTAACAGC GGCAAC. Data normalizations were performed using the 2(-Delta Delta C(T)) method.

Protein extraction and immunoblotting—Exponentially growing yeast strains were pelleted at 3220 x g for 5 mins. The supernatants were discarded and the pellets were resuspended in 200 µl of 20 % trichloroacetic acid (TCA) [20]. Then transferred to 1.5 ml tubes containing 300 µl of yeast cell extraction glass beads (0.5 mm diameter, BioSpec Cat. No. 11079105). Cells were lysed using a bead mill homogenizer (BeadMill 4, FisherScientific) at 5 m/sec for 5 sec and repeated 10 times. The supernatants were transferred to new 1.5 ml Eppendorfs, then the beads were topped up with 150 µl of 5% TCA and re-homogenized in the bead mill homogenizer at 5 m/sec for 5 sec and repeated 10 times. The supernatants were combined with the previous 200 µl from the initial extracts. The collected TCA extracts were centrifuged for 10 mins at 10,000 rpm (or 9391 x g) using an Eppendorf microcentrifuge at 4 ^oC. The supernatants were discarded and the remaining pellets were washed once in 70% ethanol to remove residual TCA. The pellets were resuspended in 100 µl of 1 X SDS loading buffer. The extracts will turn yellow colour because of the pH change. The pH was restored by adding 5 µl of 1 M Tris base solution that was not pH adjusted. Protein samples were loaded on SDS-PAGE gels. Separated proteins were transferred to 0.22 µm nitrocellulose membranes, presoaked in transfer buffer (48 mM TRIS, 390 mM Glycine, 20 % methanol, and 1% SDS) using the Trans-Blot Turbo transfer system at 25 V for 30 mins. Membranes were blocked in 5 % non-fat milk in TBS-Tween (10 mM Tris-HCl pH 7.5, 15 mM NaCl, 1.2 mM EDTA, and 0.1 % Tween 20) for 1 hr, then incubated with the indicated antibodies overnight at 4^oC. Antibodies used in the study were anti-Phospho-p44/42 MAPK (Erk1/2) Thr202 /Tyr204 (rabbit mAB 4370, Cell Signaling) generously provided by Dr. Essam Abdelalim (Qatar Biomedical Research Institute, Qatar), anti-GFP IgG (Roche antibodies), and anti-PAP (Sigma-Aldrich, P1291, St. Louis, MO, USA). The following day membranes were washed with TBS-Tween three times for 5 mins each then probed with HRP-Affinity pure (H+L) secondary antibodies 1:5000 (Jackson Immunoresearch) for 1 hr at room temperature. Membranes were visualized using Pierce™ ECL Western Blotting Substrate (Thermofisher Scientific).

FLAG-H2B purification by anti-FLAG affinity gel—Cell pellets from exponentially growing cells in YPD medium were resuspended in 4 volumes of native lysis PBS buffer containing (5 mM EGTA, 5 mM EDTA, 0.5% Triton X-100, 0.5% Nonidet-P40, 10% glycerol, 50 mM sodium fluoride, 10 mM β-glycerophosphate, 5 mM sodium pyrophosphate, 5 mM sodium orthovanadate, 1× protease inhibitor cocktail, 2 mM PMSF) and lyzed by mechanical shearing using acid-washed glass beads as previously described [26]. After separation from glass beads and centrifugation at 16,000× g for 10 mins at 4 °C, the supernatant was incubated with anti-FLAG M2 affinity gel (Sigma) for 3 hrs at 4°C, and then washed with native lysis PBS buffer and TBS (10 mM Tris-HCl pH 7.5 and 15 mM NaCl), three times each. Immunoprecipitates were eluted by elution buffer (50 mM Tris-HCl, pH 7.5, 10 mM EDTA, 1% SDS) for 20 min at 42 °C [26].

Mass spectrometry—Polypeptide bands were excised from the silver-stained gels and subjected to micro-capillary LC/MS/MS analysis mass spectrometry for identification and or modifications (Taplin Mass Spectrometry Facility, Harvard Medical School, Boston, MA, USA).

Cell cycle analysis—Overnight cultures were sub-cultured for 3 to 4 hrs, samples were taken as untreated controls, and then the cells were treated with either α-factor or rapamycin (see figure legends). Following the treatment, the cells were washed and placed in fresh media to allow for recovery. During the recovery phase, samples were taken at the indicated times for cell cycle analysis as previously described [27].

Hot phenol extraction to prepare yeast RNA for Microarray using Affymetrix arrays—

Exponential cultures (50 ml of OD₆₀₀ = 0.7) were either untreated or treated with rapamycin (200 ng/ml for 30 mins), cells harvested (4,000 rpm (3220 x g) for 2 min), resuspended in 6 ml of ice-cold sterile H₂O, immersed into liquid nitrogen to snap freeze the cell pellet followed by immediate storage at -80°C. The next day, the cell pellet was thawed on ice, and total RNA was extracted using the hot phenol extraction protocol [28].

Microarray data analysis—Microarray analysis was performed using Affymetrix GeneChip® Microarray at Genome Québec Innovation Centre and McGill University. The Affymetrix raw data “.CEL” files were imported into the FlexArray (version 1.6.3) followed by execution of robust multi-array average (RMA), which performs the background correction and quantile normalization. Principal components analysis (PCA) was used as a tool to perform quality control for the data. For subsequent statistical analysis, we used the cyber-T (Baldi & Long), Bayesian framework implemented in Flex Array. Genes up-regulated (≥ 2 fold change) and down-regulated (≤ 0.5 fold change) with high statistical significance (p-value ≥ 0.01) were exported as text files (“.TXT”) for further analysis. Volcano plots of the differentially expressed genes were generated using –Log₁₀ (p-value) and Log₂ (Fold change). Venny 2.0.2 (Computational Genomic Services, CSIC) was employed for comparing gene lists and drawing Venn’s diagram. Functional annotation clustering of the differentially expressed genes related to biological pathways was then performed using Gene Ontology (GO) term enrichment analysis and KEGG pathway mapping through DAVID Bioinformatics Resources 6.7 (http://david.abcc.ncifcrf.gov) with ease score = 0.01 and similarity threshold = 0.50. GO terms significantly represented among differentially expressed genes were then listed with their corresponding p-value and FDR in Supplementary Table II. False discovery rates were controlled using the Benjamini Hochberg method. GO annotation of genes was obtained from the Affymetrix database.

Identification of histone mutants with altered cellular response to rapamycin—A collection of 442 yeast strains expressing mutated versions of the core histones were created by replacing each amino acid residue of H2A, H2B, H3, and H4 with alanine. The individual variant carried by a single copy plasmid was introduced into a modified parental strain deleted for both copies of the respective endogenous histone genes [24]. We screened the entire histone mutant collection to identify those that were either sensitive or resistant to rapamycin using spot test analysis. This screen identified a single mutant H2A E65A showing sensitivity to rapamycin, as compared to the WT (Fig. 1A). However, this H2A E65A mutant also showed sensitivity to several other agents such as the DNA damaging agents methyl methanesulfonate (MMS) and 4-nitroquinoline-1-oxide (4-NQO)(data not shown), suggesting that H2A E65A might affect multiple cellular functions. In addition, the screen identified eight mutants displaying variable degrees of resistance to rapamycin when compared to the strains expressing WT histones (Fig. 1A). The eight rapamycin-resistant mutants did not show cross-resistance towards other drugs including the DNA damaging agents MMS and 4-NQO, as well as the environmental toxic metalloid arsenite (data not shown), suggesting that these histone residues may be specifically responding to rapamycin.

The histone mutants that were resistant to rapamycin and showed WT responses to other agents were found within histones H2B, H3, and H4, and none was recovered from the set of H2A alleles (Fig. 1). Only one mutant, H2B R95A, was recovered from the histone H2B collection that exhibited prominent resistance to rapamycin amongst all the histone mutants when tested semi-quantitatively by the spot test analysis (Fig. 1A). This H2B R95A mutant was independently checked for growth rate in liquid culture by assessing for cell density at OD 600 throughout 12 hrs in the absence and presence of rapamycin. The H2B WT and H2B R95A mutant cells proliferated at the same rate in the absence of rapamycin (Fig. 1B). However, in the presence of rapamycin growth of the H2B WT was significantly impaired by 2.5 hrs, while the H2B R95A mutant continued to grow (Fig. 1B). This latter analysis is consistent with the H2B R95A mutant being defective in a process that attenuates cell growth upon exposure to rapamycin.

In the case of histone H3, only three rapamycin-resistant mutants H3 G12A, H3 V46A, and H3 E94A were recovered, although these were not as resistant to rapamycin as H2B R95A (Fig. 1A). The H4 mutants (R19A, I21A, L22A, and R36A) were located primarily in the N-terminal part of the protein. The H4 L22A mutant was more resistant to rapamycin as compared to H4 R19A, H4 I21A, and H4 R36A and appeared to be as resistant as the H2B R95A mutant (Fig. 1A). It is noteworthy that the N-terminal tail of H4 makes contact with the H2A-H2B dimer, and plays a major role in many processes including replication-coupled chromatin assembly and gene expression [29]. Collectively, it appears that a narrow set of histone residues can specifically cause resistance to rapamycin when replaced with alanine. Since the histone H2B R95A mutant was strikingly resistant to rapamycin and did not display sensitivity or resistance to other agents [23], we focused on unraveling its role in response to rapamycin.

Microarray analysis reveals that H2B R95A downregulates several genes in the pheromone pathway—To obtain molecular insights into how H2B R95A brings about rapamycin resistance, we compared the gene expression pattern of the H2B R95A mutant with the H2B WT under normal growth conditions and when the cells were treated with rapamycin (200 ng/ml for 30 mins). A volcano plot of genes differentially expressed under normal conditions revealed that 25 genes, mainly belonging to ribosome biogenesis and RNA processing, were upregulated (P-value of ≤ 0.01) in the H2B R95A mutant as compared to the WT (Fig. 2A, shown in red). More than 50 genes were downregulated in the mutant as compared to the WT (Fig. 2A, shown in green), and of these, 26 belong to the pheromone response pathway [30]. These results suggest that the Arg95 residue of H2B plays a predominant role to ensure proper regulation of the pheromone pathway genes, consistent with the observation of Dai et al that this mutant has a defect in mating [31].

Rapamycin did not affect the expression profile of these pheromone pathway genes in the H2B WT or H2B R95A mutant using two-dimensional hierarchical clustering (Supplementary Fig. S1). This analysis grouped the non-treated and rapamycin-treated WT and the H2B R95A mutant in distinct clusters, implying that rapamycin did not affect the expression profile of these pheromone pathway genes (Fig. 2B).

We further analyzed the data by comparing genes that were differentially expressed between the WT and the H2B R95A mutant following rapamycin treatment using Venn diagrams (Fig. 2C). The analysis showed that rapamycin treatment caused up-regulation of 70 genes in the H2B R95A mutant and 21 in the H2B WT, with 14 being common to both strains (Fig. 2C). In contrast, a considerable number of genes (354) were significantly down-regulated in the H2B R95A mutant and 86 in the H2B WT with 81 being common to both strains (Fig. 2C). Almost all the differentially expressed genes in the H2B R95A mutant were enriched in the same GO term as the H2B WT and related, e.g., to ribosome biogenesis, RNA processing, RNA maturation, and export from the nucleus (Supplementary Table S2). This analysis suggests that the H2B R95A mutant is still capable of altering the expression of a subset of genes similar to the H2B WT in response to rapamycin.

H2B R95A mutant drastically reduces the expression of the STE5 gene and its encoded protein—In the pheromone response pathway, the scaffold protein Ste5 and its associated kinases Ste11, Ste7, Fus3, and Kss1 are recruited to the α-factor receptor Ste2 located at the plasma membrane when cells are exposed to α-factor. This brings the MAPKKK Ste11 in proximity with another membrane-bound complex containing the Ste20 kinase [30, 32, 33]. Ste20 phosphorylates Ste11 which then activates the MAPKK Ste7, which in turn activates the MAPKs Kss1 and Fus3 [30, 32, 33]. The activated Fus3 kinase translocates to the nucleus leading to the downregulation of the G₁ cyclins including Cln1 and Cln2 causing cell cycle arrest [34, 35]. Since Ste5 is a crucial component that allows the assembly and communication between the kinases, and mutants deleted for the STE5 gene cannot transmit a signal along the pheromone pathway to activate the MAPKs [33], we checked whether STE5 gene expression is indeed downregulated by H2B R95A mutant as revealed by the microarray data (Fig. 2). Total RNA was isolated from H2B WT and the H2B R95A mutant and the cDNAs derived from reverse transcriptase were used to quantify STE5 gene expression by quantitative PCR and normalized against the ACT1 gene. The analysis revealed that the STE5 gene was dramatically downregulated in the H2B R95A mutant as compared to the H2B WT, consistent with the microarray data (Fig. 3A and Fig. 2A, respectively).

We next checked whether the Ste5 protein would also be similarly downregulated in the H2B R95A mutant. To do this, we introduced a single-copy plasmid pSTE5-GFP expressing Ste5 from its promoter, as a GPF fusion protein, into the H2B WT and H2B R95A strains and monitored Ste5-GFP expression level by immunoblot analysis with anti-GFP antibodies, as no commercial Ste5 antibody is available [36]. The Ste5-GFP was highly expressed in the H2B WT strain, but only weakly expressed in the H2B R95A mutant (Fig. 3B, lane 2 vs. 5). Under the extraction conditions, some of the native Ste5-GFP protein was apparently proteolytically processed to a lower molecular weight isoform of ~ 80 kDa (Fig. 3B, shown by an asterisk). A control protein GFP-Apn1 driven from the galactose-inducible promoter GAL1 under the non-induced condition was expressed at the same level in both the H2B WT and H2B R95A strains (Fig. 3B lane 3 and 6, respectively). These findings support the notion that the pheromone response pathway is disrupted in the H2B R95A mutant.

ste5 null mutant displays resistance to rapamycin—To determine whether Ste5 is involved in controlling the cellular response to rapamycin, we used a different and most common parental background strain BY4741 and its isogenic ste5Δ mutant and test for rapamycin resistance using spot test analysis. As shown in Fig. 4, the ste5Δ mutant displayed resistance to rapamycin as compared to the parent BY4741, suggesting that Ste5 is required to channel the rapamycin signal to trigger growth arrest. Similar results were obtained when the STE5 gene was deleted from the W303 parental background (Supplementary Table S1). In contrast, the ste2Δ mutant lacking the transmembrane α-factor receptor protein Ste2 did not show resistance to rapamycin when compared to the WT (Fig. 4). Based on this observation, it would appear that Ste2 is not required for the recruitment of Ste5 and its associated proteins to the plasma membrane to signal the response by rapamycin.

Rapamycin induces G₁ arrest in the H2B WT, but not in the H2B R95A mutant—When WT cells are challenged with α-factor, the signal is transmitted along the pheromone pathway leading to cell cycle arrest in the G₁ phase[30]. If rapamycin uses this same pathway to signal G₁ arrest [10], then it is anticipated that this arrest would be disrupted in the H2B R95A mutant. Exponentially growing asynchronous H2B WT cells were treated with rapamycin (200 ng/ml for 60 mins), then washed to remove the drug, followed by post-treatment recovery in fresh media, and the samples taken at the indicated time were processed by Fluorescence-Activated Cell Sorting (FACS) analysis (Fig. 5). The H2B WT cells were rapidly arrested in the G₁ phase following the rapamycin treatment (Fig. 5A, second panel) and remained in the G₁ phase during the duration of the sampling (90 mins) in the fresh media without rapamycin (Fig. 5A, third, fourth, and fifth panels). In contrast, the asynchronous population of the H2B R95A mutant cells failed to arrest in the G₁ phase following rapamycin treatment (Fig. 5B vs. 5A). This observation is consistent with the H2B R95A mutant ability to grow in the presence of rapamycin (Fig. 1). We interpret these findings to indicate that rapamycin may transmit a signal through the pheromone response pathway to arrest the cell cycle in the G₁ phase.

In the control experiment, exponentially growing cultures were treated with α-factor for 3 hrs, washed free of the α-factor, and the cell cycle release was monitored over time post-treatment in fresh media using FACS. The asynchronous cell populations for both the H2B WT and the H2B R95A mutant showed a similar proportion of cells in the G₁ and G₂ phases (Supplementary Fig. S3A). As expected, following α-factor treatment, the H2B WT cells were arrested in the G₁ phase and re-entered the cell cycle upon removal of the α-factor (Supplementary Fig. S3A). In contrast, the H2B R95A mutant failed to arrest in the G₁ phase, even after prolonged exposure to the α-factor, and continued to progress normally in the cell cycle (Supplementary Fig. S3B). This finding confirms that the H2B R95A mutant is indeed defective in the pheromone response pathway.

Fus3, a downstream component of the pheromone pathway, is expressed in the H2B WT, but not detected in the H2B R95A mutant—The MAP kinases Kss1 (43 kDa) and Fus3 (41 kDa) are downstream components of the pheromone response pathway that can be phosphorylated[37]. Under conditions of starvation, Kss1 (43 kDa) can act on the Ste12 transcriptional activator to turn on filamentation genes[37]. Likewise, Fus3 when activated, for example, by α-factor can also regulate the function of the transcription factor Ste12 that controls expression of the mating genes leading to G₁ arrest[37]. The phosphorylated form of Kss1 and Fus3 is readily detected by immunoblot analysis when probed with anti-ERK1/2 antibodies [38]. This antibody recognizes the active phosphorylated form of Kss1 and Fus3, as well as other kinases such as Slt2 (52 kDa), which is required is to maintain the integrity of the cell wall [38]. We examined the phosphorylation status of Kss1 and Fus3 and whether these two MAPKs would be altered in the H2B R95A mutant in comparison to the H2B WT in response to rapamycin. As expected, the anti-ERK1/2 antibody detected the phosphorylated Kss1 and Fus3 in the H2B WT strain using 4 to 20 % gradient SDS polyacrylamide gel, although better resolution can be seen on standard 12 % gel (Fig. 6, lane 4 vs. lane 1). Neither of the MAPKs was visibly detected in the H2B R95A mutant as compared to the H2B WT (Fig. 6, lane 1 vs. lane 4). This latter finding is consistent with the microarray data revealing that multiple genes of the pheromone pathway, including FUS3, are downregulated in the H2B R95A mutant (Fig. 2A). Treatment of the H2B WT cells with rapamycin did not show any noticeable increase in the Kss1 or Fus3 phosphorylation status (Fig. 6 lanes 5 and 6 vs. 4), excluding the possibility that rapamycin mode of action is similar to that of α-factor triggering MAPKs activation. It is noteworthy that the anti-ERK1/2 antibody can also detect the Slt2 kinase that responds to various stress conditions including heat shock and oxidative stress [38]. The Slt2 kinase was present at nearly the same level in the H2B WT and the H2B R95A mutant, and unaffected by rapamycin treatment (Fig. 6 lanes 4 to 6 vs. lanes 1 to 3), suggesting that the H2B R95A mutant is not likely to harbor global downregulation of signaling pathways. Taken together, the above results suggest that the inability of the H2B R95A mutant to arrest in the G₁ phase in response to rapamycin is consistent with the downregulation of signaling components of the pheromone response pathway.

Rapamycin treatment accumulates the cyclin Cln2 at a higher level in the ste5Δ mutant, as compared to the WT—If rapamycin-induced G₁ arrest involves the downregulation of the G₁ cyclins (Cln1-3)[16, 17], we anticipate that such regulation would be compromised in the ste5Δ mutant allowing the cells to confer resistance to rapamycin. We examined the level of the G₁ cyclin Cln2 in the parent BY4741 strain and the isogenic ste5Δ mutant, both expressing CLN2-TAP at the endogenous locus to monitor the level of Cln2-TAP with the TAP antibody, which detects the Protein A portion of the TAP tag [39]. Briefly, the parental and ste5Δ mutant cells were grown in liquid YPD and treated in the log phase without and with an acute dose of rapamycin (200 ng/ml), samples taken at zero, 30, 60, and 120 mins, and processed by TCA extraction for immunoblot analysis. Upon rapamycin treatment, Cln2-TAP was unexpectedly induced at least 3-fold in the ste5Δ mutant within 30 mins and further accumulated by 120 mins (Fig. 7A, lanes 5 to 8 and quantified as in Fig. 7B, and supplementary Fig. S3 for another independent experiment). In contrast, there was a modest induction of Cln2-TAP in the parental BY4741 strain after 30 min of rapamycin treatment, which continued to accumulate by 120 mins (Fig. 7A, lanes 1 to 4 and quantified as in Fig. 7B, and supplementary Fig. S3), but not to the same extent as the ste5Δ mutant. While this finding suggests that there could be a strain-specific response towards rapamycin, due to the lack of downregulation of Cln2-TAP, it strongly indicates that the early upregulation of Cln2 might be associated with the resistance of the ste5Δ mutant towards rapamycin.

In the present study, we reported the identification and characterization of a variant of histone H2B, R95A, which was isolated by thoroughly screening a comprehensive histone mutant library [24] for resistance specifically to the immunosuppressant rapamycin. The H2B R95A mutant was the only one showing marked resistance to rapamycin, as compared to other mutants identified by the screen that displayed varying resistance to the drug. We used this H2B R95A mutant to investigate the molecular defects associated with the Arg95Ala substitution leading to rapamycin resistance in yeast cells. Our data revealed that the H2B R95A variant downregulated many genes of the pheromone response pathway consistent with the mutant inability to arrest in the G₁ phase in response to α-factor. Rapamycin is believed to trigger G₁ arrest by repressing the transcription as well as the degradation of the G₁ cyclins thereby blocking the G₁ to S phase transition [10, 17, 18]. The observation that the H2B R95A mutant continued to proliferate in the presence of rapamycin strongly suggests that this phenotype is associated with the downregulation of components of the pheromone response pathway. In support of this notion, cells lacking the scaffold protein Ste5, a key component of the pheromone signaling pathway, replicate the identical rapamycin-resistant phenotype as the H2B R95A mutant. As such, we conclude that the pheromone response pathway is functionally involved in relaying the rapamycin signal for the subsequent G₁ cell cycle arrest in WT cells. However, the exact link between the pheromone response pathway and the cell cycle arrest in response to rapamycin remains obscure. It is noteworthy that α-factor exposure triggers the sequential phosphorylation of the MAP kinases of the pheromone pathway including Fus3, which performs multiple functions such as repressing the expression of the cyclin genes to trigger G₁ arrest [40]. We have not observed any visible activation of the MAPKs, Kss1 and Fus3 in the H2B WT strain upon rapamycin treatment using the anti-Erk1/2 antibody that recognizes an increase in the phosphorylation of these kinases when cells are exposed to α-factor [37]. However, we cannot exclude the possibility that the unphosphorylated form of Kss1 and/or Fus3 might be required to promote rapamycin-induced G₁ arrest.

It has been established that rapamycin treatment represses the transcription and translation of the G₁ cyclins, which are normally required to target and promote degradation of inhibitors such as Whi5 and Sic1 of transcription factors ultimately setting the transcription factors free to activate gene expression [10, 16, 41]. Several studies demonstrated that rapamycin triggers the downregulation of G₁cyclins leading to G₁ arrest [16, 17]. While the downregulation of the G₁cyclins can be detected as early as 60 mins and near-complete disappearance by 240 mins, which appears to be strain-dependent [17, 18], paradoxically, we found a different response in the commonly used parental background strain BY4741. Cln2 monitored as Cln2-TAP, was significantly induced by rapamycin from 30 mins and lasted for 120 mins in the BY4741 WT strain (Fig. 7). Whereas the previous reports used synthetic complete media, we used the rich media YPD for all of our experiments, which could account for the difference in Cln2 response to rapamycin. Nonetheless, under the same growth condition cells lacking the scaffold protein Ste5 showed a substantially elevated level of Cln2 as early as 30 mins following treatment with rapamycin when compared to the modest induction seen in the WT strain. Although we did not create the endogenous Cln2-TAP tag in the H2B R95A mutant, we expect that in response to rapamycin Cln2 will be significantly elevated in this strain since it is unable to efficiently express Ste5. The higher Cln2 level upon rapamycin treatment could be due to the loss of negative feedback control in the absence of Ste5 [42]. Consequently, the elevated Cln2 could reinforce phosphorylation of the CDK inhibitor Sic1 such that it is rapidly degraded and unblock any potential cell cycle arrest caused by rapamycin [42]. This is a likely scenario as Ste5 and Sic1 possess the Leucine-Proline rich sequence required to allow docking of Cln2 to regulate the functionality of these substrates [43]. Another possibility might be to maintain the transcriptional repressor Whi5 in the hyperphosphorylated state preventing it from inhibiting the SBF transcription factor that activates CLN1 and CLN2 gene expression, thus creating a positive feedback loop that drives higher expression of Cln2 [15]. In the case of the parent, we cannot exclude the possibility that the modest increase in Cln2 level caused by rapamycin might perform a significant function such as blocking Ste5 membrane localization by Cln2-CDK [36, 44]. Nevertheless, the most significant finding from our study is the discovery that yeast cells exploit the pheromone pathway to arrest the cell cycle in the G₁ phase in response to rapamycin (Fig. 8). Reducing the expression of these MAPK genes via H2B R95A mutation would promote the expression of the G₁ cyclins and allow the cells to proliferate in the presence of rapamycin (Fig. 8).

The observation that the ste5Δ mutant, but not the ste2Δ strain lacking the α-factor receptor, displayed resistance to rapamycin, suggests that the mechanism by which rapamycin transmits a signal via the pheromone pathway precludes the recruitment of Ste5 to the Ste2 receptor on the plasma membrane as reported for α-factor. Thus, while α-factor binds to Ste2 and initiates the signal to arrest the cell cycle in G₁, rapamycin could intersect the pathway at the level of the Ste5 scaffold protein or further downstream. It is noteworthy that Ste5 is phosphorylated at eight sites within the N-terminus and these can be regulated by CDK and the MAPK Fus3 to modulate Ste5 membrane association [33, 44]. We have not seen changes in the migration pattern of Ste5-GFP in response to rapamycin, although the addition or removal of any unique phosphorylation might be technically challenging to be discerned by one-dimensional SDS-PAGE. There is evidence that during the mating signal Ste5 undergoes conformational changes to unblock its auto-inhibitory effect caused by an intramolecular interaction between two domains, the pleckstrin homology, and the von Willebrand type A, thereby allowing the activation of Fus3 [45]. It would be interesting to explore whether the inhibition of the Torc1 kinase by rapamycin intersects the pheromone response pathway to alter the phosphorylation sites within the N-terminus of Ste5 and or unblock its auto-inhibitory conformation such that it is poised to activate G₁ arrest.

We remark that the H2B R95A variant was also previously isolated in a screen for the loss of transcription repression of reporter genes embedded within the silent chromatin regions of the telomere [31]. Dai et al showed that the H2B R95A mutant lost telomeric silencing in a region that spans at least 20-kb from the end of the telomere [31]. In addition, the authors described other histone residues such as H2B K123, which is ubiquitylated and required for the di- and trimethylation of H3 K4 and H3 K79 that caused a loss in silencing at rDNA and telomeres when mutated [31]. We did not isolate from our screen the H2B K123A, H3 K4A, H3 K79A, or other known histone mutants, such as H4 K16 that lost silencing at the rDNA and telomeres, that would play a role in the resistance to rapamycin [31]. Thus, while defective silencing at the ends of the telomere may lead to other unidentified drug-resistant phenotypes, the telomeric silencing caused by H2B R95A is not associated with rapamycin resistance, otherwise, several of the histone variants causing silencing at rDNA and the telomeres would be expected to show resistance to rapamycin. We propose that the Arg95 residue of histone H2B performs multiple functions including the ability to maintain expression of the pheromone pathway genes, which are required to mount a response to rapamycin-induced cell cycle arrest.

Attempts to determine whether the Arg95 residue is modified using mass spectrometry analysis of purified H2B derived from untreated and rapamycin-treated cells did not reveal any modification. Dai et al also searched for possible Arg95 methylation and found no evidence for such modification under normal growth conditions [31]. We cannot exclude the possibility that a minor fraction of the total H2B could be methylated at Arg95, in particular since H2B R95A does not have a global effect and only affected the expression of a small number of genes. There are several examples of a unique histone modification that alters a specific set of genes, which affects a unique biological process. For example, the study by Tessarz et al used a biochemical approach and identified a single glutamine residue (Q105) of yeast H2A that is methylated by the essential Nop1 methyltransferase [46]. The H2A Q105 methylation is restricted to the nucleolus and located primarily at the 35S DNA transcription units, as compared to the entire yeast genome [46]. H2A Q105 spans a binding site for the FACT complex and H2A Q105A mutant can disrupt this binding altering transcription at the rDNA locus [46]. So far, the transcription factor(s) that is recruited by H2B Arg95 to promote expression of the pheromone response gene is not known.

Besides H2B R95A, our screen also revealed mutants that are less resistant to rapamycin such as H4 L22A. Although the N-terminal of H4 is linked to rDNA regulation, silencing of this region is not involved in rapamycin resistance. We have not explored if H4 L22A plays a minor role in activating the pheromone pathway or performs an independent function leading to rapamycin resistance. However, several other proteins are involved in rapamycin resistance such as the copper-zinc superoxide dismutase Sod1 [47]. In the absence of Sod1, it is believed that the Torc1 complex is inactivated by the elevated levels of endogenous superoxide anions leading to rapamycin resistance [47]. Since sod1Δ mutants cause oxidative damage to other metabolic enzymes [48], multiple pathways may likely co-exist besides the Torc1 complex and the downregulation of the pheromone pathway to cause rapamycin resistance.

Ethics approval and consent to participate: Not applicable

Consent for publication: All authors gave their consent for publication

Availability of data and material: Not applicable

Competing interests: All the authors declared that there are no competing interests

Funding: Qatar Foundation to the College of Health and Life Sciences, Hamad Bin Khalifa University, Education City, Doha, Qatar.

Authors' contributions: AAS, RA, MA, and DR conceived the experiments, AAS and RA conducted most of the experiments and prepared the Figures, AAS, RA, and DR analyzed the results and wrote the legends, and DR wrote most of the manuscript. All authors critically review the entire final draft of the manuscript before submission.

Acknowledgments: We thank the College of Health and Life Sciences, Hamad Bin Khalifa University, for providing scholarships to both N.N.H and N.E. The schematic representations were created using Biorender.com.

Authors’ information:

Abdallah Alhaj Sulaiman, Ph.D. Student inBiological and Biomedical Sciences, ORCID: 0000-0002-6720-9269 Email: [email protected]
Reem Ali, Ph.D. Post-Doctoral Fellow inBiological and Biomedical Sciences, ORCID: 0000-0003-2210-4241, Email: [email protected]
Mustapha Aouida, Ph.D. Research Scientist, Biological and Biomedical Sciences, ORCID: 0000-0001-7945-5320, Email:[email protected]
Dindial Ramotar, Ph.D, Professor of Biological and Biomedical Sciences, ORCID: 0000-0002-9572-7223

Email: [email protected]

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The Histone H2B Arg95 residue links the Pheromone Response Pathway to Rapamycin-Induced G1 Arrest in Yeast

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