The SAGA histone acetyltransferase module targets SMC5/6 to specific genes
Epigenetics & Chromatin volume 16, Article number: 6 (2023)
Structural Maintenance of Chromosomes (SMC) complexes are molecular machines driving chromatin organization at higher levels. In eukaryotes, three SMC complexes (cohesin, condensin and SMC5/6) play key roles in cohesion, condensation, replication, transcription and DNA repair. Their physical binding to DNA requires accessible chromatin.
We performed a genetic screen in fission yeast to identify novel factors required for SMC5/6 binding to DNA. We identified 79 genes of which histone acetyltransferases (HATs) were the most represented. Genetic and phenotypic analyses suggested a particularly strong functional relationship between the SMC5/6 and SAGA complexes. Furthermore, several SMC5/6 subunits physically interacted with SAGA HAT module components Gcn5 and Ada2. As Gcn5-dependent acetylation facilitates the accessibility of chromatin to DNA-repair proteins, we first analysed the formation of DNA-damage-induced SMC5/6 foci in the Δgcn5 mutant. The SMC5/6 foci formed normally in Δgcn5, suggesting SAGA-independent SMC5/6 localization to DNA-damaged sites. Next, we used Nse4-FLAG chromatin-immunoprecipitation (ChIP-seq) analysis in unchallenged cells to assess SMC5/6 distribution. A significant portion of SMC5/6 accumulated within gene regions in wild-type cells, which was reduced in Δgcn5 and Δada2 mutants. The drop in SMC5/6 levels was also observed in gcn5-E191Q acetyltransferase-dead mutant.
Our data show genetic and physical interactions between SMC5/6 and SAGA complexes. The ChIP-seq analysis suggests that SAGA HAT module targets SMC5/6 to specific gene regions and facilitates their accessibility for SMC5/6 loading.
Chromatin is composed of DNA and protein complexes structured at multiple levels to ensure its spatial and functional organization . Histone proteins pack DNA into nucleosomes and their arrays at the basic level. At the higher levels, structural maintenance of chromosomes (SMC) complexes (cohesin, condensin and SMC5/6) assist in the formation of high-order structures like topologically associated domains or condensed mitotic chromosomes . Chromatin compaction affects DNA accessibility at each level. Histone chaperones, modifiers, and remodelers can loosen, move or remodel nucleosomes to modulate essential processes like transcription or DNA repair [3, 4]. For example, the histone-modifying SAGA complex acetylates H3 histones at promoter regions, contributing to chromatin opening and facilitating the assembly of transcription initiation complexes onto core promoters and the recruitment of factors that directly interact with DNA .
The SMC complexes play roles in all key chromatin processes, including cohesion, condensation, replication, transcription and DNA repair. Their cores comprise the long-armed Smc, kleisin and kleisin-associated (KITE or HAWK) subunits [6, 7]. Uniquely, SMC5/6 complexes contain the highly conserved Nse1  and Nse2 ubiquitin- and SUMO-ligases, respectively [9, 10]. The Smc subunits are primarily built of head ATPase domains, long anti-parallel coiled-coil arms and hinges [11,12,13]. Two Smc molecules form stable dimers via their hinge domains, and without ATP, their arms align into rod-like structures [14, 15]. The binding of ATP molecules to the ATPase head domains promotes the formation of large annular structures [16, 17]. The ATP binding−hydrolysis cycle drives ring-to-rod dynamic changes and promotes DNA translocation or loop extrusion [18,19,20,21].
SMC complexes were believed to interact only topologically with chromatin fibres via their large ring-shaped structures, which can embrace and traverse large chromatin complexes, including nucleosomes . However, growing evidence suggests their requirement for open chromatin and direct physical binding to DNA [22,23,24]. Moreover, Piazza et al.  described the preferential binding of condensin’s kleisin-associated HAWK subunits to free DNA over nucleosomal DNA. Recent cryoEM analyses showed the formation of K-compartments within all SMC complexes, consisting of ATP-bound Smc heads, kleisin and kleisin-associated subunits, which can accommodate only free DNA [17, 25,26,27]. In line with these findings, the SAGA complex assists in loading condensin at open chromatin regions of highly transcribed genes in fission yeast . Similarly, the RSC chromatin remodelling complex recruits the Scc2-Scc4 factor to nucleosome-free regions, assisting in cohesin loading at these sites [28,29,30].
Recently, it was shown that the SMC5/6 K-compartment, composed of Smc5-Smc6 heads, Nse4 kleisin and Nse1−Nse3 kleisin-associated KITE subunits, binds free DNA [17, 22]. In our previous study, we characterized the binding of the C-terminal winged-helix (WHB) domain of Nse3 to DNA and described the essential role of Nse3-DNA interaction for SMC5/6 loading or accumulation . Here, we performed a genetic screen with a nse3-R254E fission yeast mutant that exhibits reduced DNA-binding affinity to identify new factors required for its viability. We found strong genetic interactions with the SAGA and NuA4 histone acetyltransferase (HAT) complexes. Using chromatin-immunoprecipitation (ChIP-seq) analysis, we observed a significant portion of SMC5/6 accumulated within gene regions, which was reduced in SAGA HAT deletion (Δada2 and Δgcn5) mutants. The magnitude of the decrease in SMC5/6 occupancy correlated with the SAGA-modified H3K9ac levels around the transcription start sites. The SMC5/6 reduced levels were also observed in gcn5-E191Q acetyltransferase-dead mutant, suggesting that the SAGA HAT module may target SMC5/6 to gene regions and facilitate the accessibility of chromatin for SMC5/6 loading.
Genetic screen with a DNA-binding defective allele of the SMC5/6 complex
To identify factors that facilitate the loading or accumulation of the SMC5/6 complex on chromatin, we performed a genetic search for genes affecting the survival of cells with compromised DNA-binding ability of the SMC5/6 complex . First, we created a query fission yeast strain with the DNA-binding defective nse3-R254E mutation in the PEM2 background (Additional file 1: Fig. S1A; ) and crossed it against the whole gene deletion yeast collection from BIONEER . Using yeast colony size phenotypic readout , we identified 79 deletion strains that exhibited a negative genetic interaction with nse3-R254E (Additional file 1: Table S1).
To validate our results, we randomly selected 19 of the 79 strains and crossed them with the original nse3-R254E strain . Tetrad analysis confirmed that these mutations are synthetically sick or lethal with the nse3-R254E mutation (Additional file 1: Fig. S1B). Analysis of all 79 interacting genes for the Biological process category using Gene ontologies (GO; ) showed the highest scores for DNA repair, chromatin organization, meiosis and replication processes (Fig. 1A and Additional file 1: Table S2), in line with previous studies (reviewed in [35, 36]). Reassuringly, several nse3-R254E genetic interactions overlapped with the genetic interactions of other smc5/6 mutants [22, 37,38,39,40,41,42], supporting the validity of our screen results.
Genetic interactions between SMC5/6 and histone acetyltransferase complexes
The analysis of the Cellular components GO of the 79 interacting genes showed the highest scores for histone acetyltransferase (HAT) complexes (SAGA and NuA4; Fig. 1B and Additional file 1: Table S3). Three (Ada2, Ada3/Ngg1, Gcn5) out of four HAT module subunits and one (Ubp8) out of four DUB module subunits of the SAGA complex were identified as hits in our screen . We verified their genetic interactions using tetrad analysis (Figs. 1C and S1B) and also tested the other non-essential SAGA subunits not detected in our screen. The mating defects of the Δada1, Δspt7, Δspt8 and Δspt20 deletion mutants hampered the double mutant preparation . However, the tetrad analysis of the other non-essential SAGA subunits (Additional file 1: Fig. S1C) showed negative genetic interactions with the nse3-R254E mutation (Additional file 1: Fig. S1D), suggesting a strong functional relationship between the SMC5/6 and SAGA complexes.
Interestingly, the temperature-sensitive (ts) phenotypes of the SAGA HAT module Δada2, Δada3 and Δgcn5 mutants were enhanced by nse3-R254E (Fig. 1D; ). The ts phenotypes were also enhanced by the smc6-74 and smc6-X hypomorphic mutations (Additional file 1: Fig. S2A; [38, 44]). We also used nse1-R188E and nse2-SA mutations, which specifically abrogate DNA-repair function (ubiquitin- and SUMO- ligase activity, respectively), but not the SMC5/6 essential function [8, 9]. However, these mutations did not affect the ts phenotype of Δgcn5 (Additional file 1: Fig. S2A; not shown). These data suggest that the SMC5/6 essential function supports cell survival at higher temperatures in the absence of the HAT module and, conversely, that the viability of the nse3-R254E mutant is compromised in the absence of a functional SAGA HAT module.
SMC5/6 and SAGA physically interact
The strong genetic relationship between the SAGA HAT module and the SMC5/6 complex prompted us to test their mutual physical interactions. First, we performed co-immunoprecipitation of Gcn5-myc and Nse4-FLAG kleisin subunit to show the association between the SAGA and SMC5/6 complexes in vivo (Fig. 2A). The fission yeast cells carrying Nse4-FLAG (with or without Gcn5-myc) were lysed and proteins were precipitated with an anti-myc antibody. A small amount of Nse4-FLAG was specifically recovered in the Gcn5-myc precipitates but not in the control experiment without myc-tagged Gcn5, suggesting a weak or transient association between SAGA and SMC5/6 in the yeast cells.
Next, we used our panel of yeast two-hybrid (Y2H) SMC5/6 subunits to test their interactions with the HAT module (Ada2, Ada3, Gcn5 and Sgf29) subunits. Two of the HAT module subunits, Ada2 and Gcn5, bound the Nse3 subunit (Fig. 2B and Additional file 1: Fig. S2B). The fragment analysis showed that Gcn5 bound the N-terminal part of Nse3(aa1-190), whilst Ada2 interacted with its C-terminal WHB domain (Nse3(aa200-307); Fig. 2B and Additional file 1: Fig. S2C; ). In addition, Ada2 bound the N-terminal region of Nse2 and the coiled-coil arm of Smc5 . Altogether, the Y2H data show multiple interactions between several SAGA and SMC5/6 subunits, and the co-immunoprecipitation experiment demonstrates the association between SAGA and SMC5/6 in vivo.
SMC5/6 and SAGA are required for efficient DNA repair
The SAGA complex plays an important role in transcription regulation and DNA repair by facilitating the accessibility of chromatin to transcription factors and repair proteins [43, 47,48,49,50]. Deletion mutants of most SAGA genes were sensitive to hydroxyurea (HU; ) and SAGA mutations increased the sensitivity of the smc5/6 hypomorphic mutants to HU and other DNA-damaging agents (Fig. 3A, Additional file 1: Figs. S2A, and S3A). These data suggest either a direct role of the SAGA complex in facilitating SMC5/6 access to chromatin at sites of DNA damage or its indirect, independent role.
Upon DNA damage, SMC5/6 accumulates in foci in a Brc1-dependent way [51, 52]. To assess whether SMC5/6 chromatin accessibility at these DNA-damage sites is directly facilitated by SAGA, we analysed the Nse4-GFP foci in the Δgcn5 and Δada2 mutants (Fig. 3B). We observed no difference between the frequency of cells with foci in the wild-type (WT), Δgcn5 and Δada2 after treatment with either MMS (methyl methane sulfonate) or HU. In contrast, the number of foci in the Δbrc1 mutant was strongly reduced (Fig. 3C). These results indicate no direct involvement of SAGA in SMC5/6 localization to sites of DNA damage. Instead, they suggest that the observed HU phenotype results from additive effects of the SAGA and SMC5/6 complexes during DNA-damage repair.
SAGA targets SMC5/6 to gene regions
In addition to the accessibility of chromatin to DNA repair and transcription factors, SAGA facilitates chromatin accessibility to condensin complexes . Therefore, we determined the SMC5/6 localization in the unchallenged WT, Δgcn5, Δada2 and Δubp8 cells using chromatin immunoprecipitation of Nse4-FLAG followed by deep sequencing (ChIP-seq). In the WT cells, most SMC5/6 localized to the repetitive regions (like rDNA, centromeres or tDNA copies), with the highest occupancy at the rDNA repeats (Fig. 4A) consistent with previous reports [53,54,55,56,57,58]. Interestingly, we identified 331 Nse4-FLAG peaks (representing ¼ of the total Nse4 occupancy; Fig. 4A) that localized to gene regions.
In Δgcn5 and Δada2 mutants, SMC5/6 distribution was altered, whilst SMC5/6 occupancy in the Δubp8 mutant was similar to that in WT cells. A heatmap clustering analysis showed that the Nse4-FLAG peaks were either enhanced, unchanged or reduced in the Δgcn5 and Δada2 mutants (Fig. 4B). The peaks were mainly enhanced at the repetitive sequences (Fig. 4C), whilst most peaks in the intergenic regions were not changed (Fig. 4D). Strikingly, most peaks within the gene regions showed reduced Nse4 occupancy (252 out of 331; Fig. 4C and D), suggesting that the SAGA HAT module targets SMC5/6 to gene loci.
SAGA plays a role in facilitating chromatin accessibility to SMC5/6 in specific regions
The SAGA HAT module acetylates histone H3 at its lysine K9 and K14 residues [59, 60]. To determine the H3K9ac distribution in our fission yeast cells, we performed ChIP-seq using an anti-H3K9ac antibody. A heatmap clustering analysis showed that the magnitude of decrease in SMC5/6 occupancy in gene bodies in the Δgcn5 mutant (Δgcn5-WT plot; Fig. 5A and B) correlated with H3K9ac levels around the transcription start site and with transcript levels . It suggests that the SAGA-dependent H3K9 acetylation may facilitate the accessibility of chromatin to SMC5/6 at gene regions.
To assess the role of the SAGA-dependent acetylation further, we used the gcn5-E191Q acetyltransferase-dead mutant . First, we found that the gcn5-E191Q ts phenotype was exacerbated by nse3-R254E, similar to Δgcn5 (Additional file 1: Fig. S3D). Second, the gcn5-E191Q nse3-R254E double mutant was as sensitive to DNA-damaging agents as the Δgcn5 nse3-R254E double mutant. Finally, using ChIP-qPCR analysis, we observed reduced Nse4-FLAG occupancy in the gcn5-E191Q mutant at selected gene regions similar to Δgcn5 (Fig. 5C), although some loci exhibited only a modest drop in SMC5/6 levels. Altogether, our results suggest an important role for the SAGA HAT module in targeting and facilitating the accessibility of chromatin to SMC5/6 at gene loci.
Here, we showed a new functional partnership between SAGA and SMC5/6 complexes. These complexes exhibited negative genetic interactions and physical associations mediated via multiple protein–protein interactions. Gcn5 deletion reduced SMC5/6 occupancy specifically at the gene regions but did not affect the formation of SMC5/6 foci upon DNA damage.
It was recently shown that plant ADA2b binds SMC5 and assists in the localization of SMC5/6 to DNA-damage sites . Later studies uncovered an ADA2b-diRNA pathway, involving specifically ADA2b without the other SAGA subunits, targeting SMC5/6 to DNA-damage foci in plants . In contrast, our Y2H results show multiple interactions between several SAGA and SMC5/6 subunits (Fig. 2B). In addition, our co-immunoprecipitation experiment shows indirect interaction between Nse4-FLAG and Gcn5-myc subunits. As Nse4-FLAG and Gcn5-myc proteins incorporate into their respective complexes normally (Additional file 1: Fig. S4A; ), their co-immunoprecipitation confirms the association between SAGA and SMC5/6 complexes in vivo (Fig. 2A).
Furthermore, we and others showed that the SMC5/6 targeting to DNA-damage sites depends on the BRCT domain-containing Brc1 protein but not on Ada2 or Gcn5 (Fig. 3; ) in fission yeast, suggesting a plant-specific function of the ADA2b-SMC5 interaction in DNA-damage response. Future studies may show if SAGA likewise facilitates the accessibility of chromatin to SMC5/6 at gene loci in plants. Interestingly, we found an interaction between human hTADA2B and hNSE4a/b subunits (Additional file 1: Fig. S2D), suggesting that physical association between the SAGA and SMC5/6 complexes is conserved. It will be interesting to examine the functional relationships between human SAGA and SMC5/6 complexes, and explore the SAGA-SMC5/6 relationship further.
Consistent with the lack of effect of SAGA on SMC5/6 localization to sites of DNA damage, the SMC5/6 levels at repetitive regions (which are prone to DNA damage even without any genotoxic treatment) were not reduced in Δgcn5 and Δada2 deletion mutants (Fig. 4). In our ChIP-seq experiments, the repetitive loci were instead enriched for SMC5/6 upon SAGA HAT deletion. As the SMC5/6 accumulation at repetitive regions depends on H3K9 methyltransferase Clr4 in fission yeast , we speculate that reduced acetylation levels promoted an increase in methylation levels upon gcn5 acetyltransferase deletion, indirectly stimulating the SMC5/6 localization to repetitive heterochromatic regions .
Interestingly, enhanced SMC5/6 accumulation at repetitive regions could not rescue smc5/6 phenotypes. Instead, smc5/6 saga double mutants exhibited additive growth defects, suggesting that either increased SMC5/6 accumulation at repetitive regions is toxic or reduced SMC5/6 loading at gene regions exacerbates smc5/6 problems. Although we cannot exclude the former indirect effect, we found the latter possibility more straightforward. In this case, the reduced SMC5/6 targeting to gene regions upon gcn5 deletion would exacerbate the DNA-binding defect of the nse3-R254E mutant, resulting in a more severe double mutant phenotype (Fig. 1).
Based on our data, we propose the following model for SAGA-dependent loading of SMC5/6: 1. SAGA binds SMC5/6 and targets it to specific gene regions; 2. H3K9 acetylation further helps open chromatin to allow SMC5/6 K-compartment physically bind DNA (Fig. 6). Interestingly, the SMC5/6 subunits (Nse2, Nse3 and Smc5 arm) are aligned at the surface of the rod-shaped complex for binding to the SAGA complex (Fig 2B and Additional file 1: Fig. S4B; ). In contrast, the Nse3 subunit is mostly buried inside the ring-shaped complex (Additional file 1: Fig. S4C; ), and its C-terminal WHB domain is directly bound to DNA. Therefore, we hypothesize that SAGA binds rod-shaped SMC5/6 first and brings it to its target gene region (Fig. 6, targeting step). At the target regions, SAGA acetylates H3 histones and facilitates further chromatin opening. This positions SMC5/6 to close proximity to free DNA and stimulates its direct binding to DNA. Nse3 binding to DNA results in the conformational change to the ring shape and complete or partial dissociation from the SAGA complex (Fig. 6, DNA-binding step).
This model implies that SMC5/6 loading is primarily dependent on the SMC5/6 binding to SAGA (Fig. 6, targeting step). The second DNA-binding step requires free DNA. This step depends on the open state of the chromatin, which might already be present at the target region (independent of SAGA) or induced by Gcn5-mediated histone acetylation. This two-step model explains different SMC5/6 levels in gcn5 deletion and gcn5-E191Q mutant at different loci (Fig. 5C). Loading of SMC5/6 is already blocked in the first step in gcn5 deletion, resulting in reduced SMC5/6 accumulation. In the acetyltransferase-dead gcn5-E191Q mutant, SAGA binds SMC5/6 and brings it to the target region in the first step, whilst the SMC5/6 binding to DNA depends on the chromatin state at particular loci. Open state of some loci may entirely depend on SAGA HAT activity, then SMC5/6 DNA binding is blocked in gcn5-E191Q (Fig. 6, middle panel), similar to gcn5 deletion (Fig. 5C, vht1 locus). Other loci may provide free DNA sufficient for SMC5/6 loading even without Gcn5-assisted chromatin opening in gcn5-E191Q (loci with only modestly or partially reduced SMC5/6 levels in Fig. 5C, like tef3 locus). Future studies will address the detailed mechanism of SMC5/6 loading.
Here we described the new role of the SAGA complex in targeting SMC5/6 to specific gene regions, which is likely mediated via multiple direct interactions between subunits of these two complexes. In addition, SAGA may further assist in SMC5/6 chromatin loading through its acetyltransferase activity. Our new findings support previous views that different factors target SMC5/6 to different genomic regions [35, 52, 53, 65]. For example, Brc1 targets SMC5/6 to DNA-damage sites via its interaction with phosphorylated H2A (the equivalent of the targeting step in Fig. 6; ). Although it is not clear how SMC5/6 reaches free DNA in this case, nucleosome-free DNA structures are known to be available during DNA-damage repair. In comparison, SAGA targets SMC5/6 to unchallenged chromatin and can also assist in providing free DNA for SMC5/6 loading via chromatin acetylation. This SAGA-dependent loading likely constitutes a more general mechanism, as SAGA was also shown to assist in loading condensin in fission yeast . In conclusion, our data outline the interplay between two key chromatin complexes, SMC5/6 and SAGA.
Standard fission yeast genetic techniques were used . Yeast strains were crossed and sporulated either at 25 °C (ts mutants) or 28 °C (non-ts mutants). Tetrad analysis was carried out on Singer MSM300 (Singer, UK). The deletion integrations were verified on both ends by PCR with specific primers to the G418 cassette and genomic sequence of a deleted gene (approximately 600–800 bp from start or end). The PCR products were sequenced.
Schizosaccharomyces pombe cultures were grown to the mid-log phase, and serial tenfold dilutions were spotted onto rich media with the indicated dose of DNA-damaging agent (hydroxyurea or methyl methane sulfonate). Subsequently, plates were incubated at the indicated temperatures (25, 28 or 37 °C) for 3–4 days. At least three independent drop tests were carried out, whilst only one representative plate was displayed in the figure. Selective media were supplemented with Nourseothricin (cloNAT, 100 μg/ml, Jena Bioscience), G418 (100 μg/ml; Applichem) and/or cycloheximide (100 μg/ml; Sigma).
Yeast genetic screens
The pAW8-Nse3 integration construct  was modified for use in the PEM2 strain as follows. The SphI site was mutated to XhoI using a site-directed mutagenesis kit (Agilent Technologies; primers: LJ48 and LJ49; Additional file 1: Table S4). The cloNAT cassette was amplified (LJ42 and LJ43) and inserted into the XhoI site in front of the Nse3 gene using the In-fusion cloning kit (Takara). A 650 bp-long genomic sequence (upstream of Nse3; LJ44 and LJ45) was inserted in front of the cloNAT cassette (using XhoI) to ensure its proper integration into the S. pombe genome. The mutant cloNAT-nse3-R254E construct was created using site-directed mutagenesis (R254E_F and R254E_R primers; ). For the yeast transformation, the WT and mutant cloNAT constructs were cleaved by SpeI, and the 3246 bp long fragment was purified from agarose gel by Gel Extraction Kit (Qiagen). Approximately 1 μg of purified DNA was transformed into the PEM2 strain  by standard LiAc protocol. The proper integration of the cloNAT-Nse3 cassette and rlp42 mutation was checked by PCR and sequencing. The nse3-R254E PEM2 strain phenotypes were compared with the original nse3-R254E strain (Additional file 1: Fig. S1A; ).
The WT and nse3-R254E mutant PEM2 strains (YLJ222 and YLJ228; Additional file 1: Table S5) were crossed with the S. pombe haploid deletion library (BIONEER, version 5, https://us.bioneer.com) according to the published protocol . The screen was repeated twice using the Rotor HDA robot (Singer, UK). The plate images were taken by a Canon EOS Rebel T3i camera, and the individual colony size was measured. The viability of single deletion mutants (control WT plates) against double mutants (test nse3-R254E plates) was compared using SGAtools online platform . Genes with a score less than − 0.25 were chosen as potential negative interactors (Additional file 1: Table S1).
The resulting group of 79 genes was analysed by the Gene ontology tool BiNGo , which is a plugin of the Cytoscape online platform . The genes were classified according to the Pombase GO database into Biological processes and Cellular component categories, respectively . The default parameters with a 0.05 significance level were applied for both categories.
Yeast two-hybrid analysis
The Gal4-based Y2H system was used to analyse SMC5/6-SAGA interactions . S. pombe ada2, ada3, gcn5 and sgf29 genes were PCR amplified from genomic DNA (primers used for ada2 and gcn5 cloning are listed in Additional file 1: Table S4). All inserts were cloned into respective sites of the pGBKT7 or pGADT7 vectors using the In-Fusion cloning system. pGBKT7-Nse2(aa2-178) was described in . pGADT7-Nse3(aa1-190) was prepared by mutagenesis of 191st aa to STOP codon in pGADT7-Nse3(aa1-328) . The Nse3(aa200-307) fragment was cut out from pTriEx4-Nse3(aa200-307)  by NcoI-XhoI enzymes and cloned into pGADT7. The Smc5(aa170-225 + 837-910) fragment was amplified from the Smc5(aa2-225 + 837-1065) construct  and inserted into the NcoI-NotI sites of pGBKT7.
The pairs of pGBKT7 and pGADT7 constructs were co-transformed into the Saccharomyces cerevisiae PJ69–4a strain by standard LiAc transformation protocol and selected on SD-Leu, -Trp plates. Drop tests were carried out on SD-Leu, -Trp, -His (with 0.3, 0.5, 1, 3, 5 or 10 mM 3-aminotriazole) plates at 28 °C. Each combination of partners was co-transformed and tested at least twice.
Co-immunoprecipitation of S. pombe proteins
Logarithmically growing YLJ507 and MMP21 cells (Additional file 1: Table S5, Fig. S3B) were cultivated in a rich medium at 28 °C (OD595 = 0.4–0.7). 5 × 108 cells were harvested by centrifugation (3 min, 4 °C, 5000 rpm) and washed with 10 ml of ice-cold PBS. Pellets were stored in the 2 ml screw cup tubes at − 80 °C. The crude yeast extracts were prepared in 400 μl CHIP lysis buffer (50 mM HEPES, pH 7.5, 140 mM NaCl, 1 mM EDTA, 1% Triton X-100, Complete EDTA-free protease inhibitor cocktail tablets, Roche) with half volume of glass beads (Sigma) in 2 ml low binding tubes using FASTprep-24 (MP Biomedicals; 5 times, 30 s, 6.5 speed). The suspension was recovered by piercing the bottom of the tube with a needle, placing it into a new 2 ml tube, and centrifugation (3 min, 4 °C, 5000 rpm). The beads were washed with 200 μl of CHIP lysis buffer (3 min, 4 °C, 5000 rpm). The collected suspensions were clarified by centrifugation (15 min, 4 °C, 15,000 rpm), and the supernatant was transferred to new low-binding tubes. 40 μl of cell extract was taken for input control. Immunoprecipitation was carried out by adding 2 μl mouse anti-myc antibody (2276S, Cell Signalling) to the cell extracts and incubation for 2 h at 4 °C. 20 μl of protein G-coated Dynabeads (Invitrogen) were washed twice with 1 ml CHIP lysis buffer and resuspended in 60 μl of CHIP lysis buffer, then added to the extract with anti-myc antibody and incubated overnight at 4 °C. The beads were pelleted using a magnetic rack, and the unbound fraction (40 μl) was taken. Beads were washed four times with 1 ml CHIP lysis buffer, and proteins were eluted by 40 μl of 1× SDS loading buffer. After 15 min incubation at room temperature, the supernatant (bound fraction) was recovered. All fractions were analysed by western blotting using mouse anti-myc-HRP (R951-25, Thermo Fisher) and mouse anti-FLAG-HRP (F1804-1MG, Sigma) antibodies, respectively.
The AlphaFold tools [72, 73] were used to generate in silico fission yeast SMC5/6 subunits and complex models. Structural models were analysed as previously described [6, 74]. Structures were visualized using PyMOL Molecular Graphics System.
Chromatin-immunoprecipitation analysis (ChIP)
All strains (Additional file 1: Table S5) were cultivated into the mid-log phase (OD = 0.4–0.6) and incubated with 1% formaldehyde for 15 min at room temperature to cross-link DNA–protein complexes. Glycine was added to a final concentration of 125 mM, and the incubation continued for 5 min. 5 × 108 cells were harvested and washed with 10 ml of ice-cold PBS. The yeast cell wall breakage was performed in 400 μl CHIP lysis buffer with half the volume of glass beads in 2 ml low-binding tubes using FASTprep-24. The suspension was washed two times with CHIP lysis buffer (15 min, 4 °C, 15,000 rpm), and 300 μl of the extract was sonicated with Bioruptor (Diagenode, 30 s ON/30 s OFF, High Power, 25 times) and clarified by centrifugation (15 min, 4 °C, 15,000 rpm), resulting in an average DNA fragment size of 300–500 bp. 5 μl of the sonicated precleared extract was taken as an input control sample.
Monoclonal anti-FLAG M2 antibody (F1804, Sigma) was diluted 1:150, incubated with precleared cell extract in 1.5 ml low-binding tube for 2 h on ice and precipitated overnight with Dynabeads protein G (Invitrogen). Precipitates were washed with 1 ml of CHIP lysis buffer, 1 ml of High Salt buffer (CHIP lysis buffer with 500 mM NaCl), 1 ml of Wash buffer (10 mM Tris–HCl at pH 8.0, 0.25 M LiCl, 0.5% NP-40, 1 mM EDTA) and 1 ml of TE buffer (20 mM Tris–HCl at pH 8.0, 1 mM EDTA). After elution (50 mM Tris at pH 8, 0.1% SDS, 10 mM EDTA) and de-crosslinking overnight at 65 °C, the DNA was purified using QIAquick PCR Purification Kit (Qiagen).
For ChIP-seq analysis, the input DNA samples were tested for DNA fragmentation and determination of DNA concentration by the Fragment analyser (Agilent). Input and immunoprecipitation (IP) samples with the best fragmentation and high concentration were used for the creation of NGS libraries (NEBNEXT ULTRA II DNA Library Prep kit, NEB) and sequencing (Illumina Next seq 500, Illumina).
Two independent replicates were performed. Cells were grown to the exponential phase (OD600 = 0.5) in the complex YES medium and fixed by adding formaldehyde to the final concentration of 1%. After 30 min incubation, the remaining formaldehyde was quenched by 125 mM glycine. Cells were washed with PBS and broken with glass beads. Extracted chromatin was sheared with the Bioruptor sonicator (Diagenode) using 15 or 30 cycles (for biological replicate 1 and 2, respectively) of 30 s ON/30 s OFF at high power settings. For all immunoprecipitations (IP) within a biological replicate, the same amount of chromatin extract was used (2.5 or 3.7 mg of total protein); 1/10 of the total chromatin extract amount was kept for input DNA control. For each IP, 5 μg of antibody (H3: Ab1791, H3K9ac: Ab4441, all Abcam) were incubated with the chromatin extract for 1 h at 4 °C with rotation. Then, 50 μl of BSA-blocked Protein A-coated magnetic beads (10002D, ThermoFisherScientific) were added to the chromatin extract-antibody suspension and incubated for additional 4 h at 4 °C with rotation. The precipitated material and input chromatin extract were de-crosslinked and treated with RNase A and proteinase K. DNA was purified using phenol–chloroform extraction and sodium acetate/ethanol precipitation. In biological replicate 2, DNA purification on AMPure XP beads (AC63880, Beckman Coulter) was performed after the phenol–chloroform extraction to remove low-molecular fragments and RNA. DNA concentration was measured using the Quantus fluorometer (Promega) and fragment size distribution was checked on Agilent Bioanalyser using the High Sensitivity DNA Assay. Library construction and sequencing (50 nt SE) were performed by BGI Tech Solutions (Hong Kong) using the BGISEQ-500 sequencing system.
NGS data analysis
The reference fission yeast S. pombe genome (2018-09-04) and annotation (2019-11-15) were downloaded from PomBase (https://www.pombase.org/; [68, 75]). Read quality was checked using FastQC version 0.11.8 (https://www.bioinformatics.babraham.ac.uk/projects/fastqc/), and reads were aligned to the S. pombe genome using HISAT2 2.1.0  and SAMtools 1.9 [77, 78]. Read coverage tracks (i.e. target protein occupancy) were then computed and normalized to the respective mapped library sizes using deepTools 3.5.1 . The raw ChIP-seq data are available from the ArrayExpress (https://www.ebi.ac.uk/) database under the accession numbers E-MTAB-11081 and E-MTAB-12401.
WT fission yeast RNA-seq data were obtained from the NCBI Sequence Read Archive (https://www.ncbi.nlm.nih.gov/sra; datasets SRR8742773-SRR8742775; ). Reads were processed and analysed with the same tools as above. All relevant scripts for (ChIP-seq and RNA-seq) data processing and analysis are available from https://github.com/mprevorovsky/Palecek-Nse-SAGA.
The Nse4-FLAG strains (crossed with the Δgcn5 or gcn5-E191Q strain; Additional file 1: Table S5) were used. The untagged wild-type strain was used as a negative control. All cells were cultivated into the mid-log phase. Cells were then incubated with 1% formaldehyde for 10 min at room temperature to cross-link DNA–protein complexes. Chromatin immunoprecipitation was performed using a protocol described above for H3K9ac ChIP with the following modifications. Monoclonal anti-FLAG M2 antibody (F1804; Sigma) was diluted at 1:350 (5 µg/sample), incubated with 2 mg of total cell extract for 2 h at 4 °C with rotation and precipitated with Dynabeads protein G (Invitrogen). After overnight incubation, several washes, elution and de-crosslinking, the DNA was purified using phenol/chloroform method.
The relative amount of PCR product was quantified by qPCR using SensiFASTTM SYBR® Hi -ROX Kit (Bioline). The sequences of primers used for the quantitative detection of the chromosomal loci are listed in Additional file 1: Table S6. Input DNA recovery was calculated as 2 squared [CT(input) − CT(immunoprecipitate)] and normalized to a negative locus slx9. Melt curve analysis was performed for each sample after PCR amplification to ensure that a single product was obtained.
For the Nse4-GFP foci number determination, cells were grown in YES medium overnight, diluted to OD = 0.4 in the morning and treated with 0.03% MMS or 20 mM HU for 5 h at 30 °C. 2.5 μl of cell culture was mounted on the slides and GFP fluorescence was observed. Pictures were taken on the Axio Imager Z1 microscope, using a Plan-Apochromat 63× oil objective, the Axiocam CCD camera and processed with the AxioVision software (all by Zeiss). A minimum of 500 cells were counted in three independent experiments. For statistical evaluation, p-values were calculated using the χ2 test.
Availability of data and materials
All relevant data are within the manuscript and its Additional files.
Uhlmann F. SMC complexes: from DNA to chromosomes. Nat Rev Mol Cell Biol. 2016;17(7):399–412. https://doi.org/10.1038/nrm.2016.30. (Epub 2016/04/14).
Davidson IF, Peters JM. Genome folding through loop extrusion by SMC complexes. Nat Rev Mol Cell Biol. 2021;22(7):445–64. https://doi.org/10.1038/s41580-021-00349-7. (Epub 20210325).
Ransom M, Dennehey BK, Tyler JK. Chaperoning histones during DNA replication and repair. Cell. 2010;140(2):183–95. https://doi.org/10.1016/j.cell.2010.01.004.
Morrison AJ, Shen XT. Chromatin remodelling beyond transcription: the INO80 and SWR1 complexes. Nat Rev Mol Cell Biol. 2009;10(6):373–84. https://doi.org/10.1038/nrm2693.
Helmlinger D, Tora L. Sharing the SAGA. Trends Biochem Sci. 2017;42(11):850–61. https://doi.org/10.1016/j.tibs.2017.09.001. (Epub 2017/09/27).
Palecek JJ, Gruber S. Kite proteins: a superfamily of SMC/Kleisin partners conserved across bacteria, archaea, and eukaryotes. Structure. 2015;23(12):2183–90. https://doi.org/10.1016/j.str.2015.10.004.
Wells JN, Gligoris TG, Nasmyth KA, Marsh JA. Evolution of condensin and cohesin complexes driven by replacement of Kite by Hawk proteins. Curr Biol. 2017;27(1):R17–8. https://doi.org/10.1016/j.cub.2016.11.050.
Kolesar P, Stejskal K, Potesil D, Murray JM, Palecek JJ. Role of Nse1 subunit of SMC5/6 complex as a ubiquitin ligase. Cells. 2022;11(1):13. https://doi.org/10.3390/cells11010165.
Andrews E, Palecek J, Sergeant J, Taylor E, Lehmann A, Watts F. Nse2, a component of the Smc5-6 complex, is a SUMO ligase required for the response to DNA damage. Mol Cell Biol. 2005;25(1):185–96. https://doi.org/10.1128/MCB.25.1.185-196.2005.
Zhao X, Blobel G. A SUMO ligase is part of a nuclear multiprotein complex that affects DNA repair and chromosomal organization. Proc Natl Acad Sci USA. 2005;102(13):4777–47782. https://doi.org/10.1073/pnas.0500537102.
Gligoris T, Löwe J. Structural insights into ring formation of cohesin and related smc complexes. Trends Cell Biol. 2016;26(9):680–93. https://doi.org/10.1016/j.tcb.2016.04.002. (Epub 2016/04/28).
Hassler M, Shaltiel IA, Haering CH. Towards a unified model of SMC complex function. Curr Biol. 2018;28(21):R1266–81. https://doi.org/10.1016/j.cub.2018.08.034.
Nasmyth K, Haering CH. The structure and function of SMC and kleisin complexes. Annu Rev Biochem. 2005;74:595–648. https://doi.org/10.1146/annurev.biochem.74.082803.133219.
Alt A, Dang HQ, Wells OS, Polo LM, Smith MA, McGregor GA, et al. Specialized interfaces of Smc5/6 control hinge stability and DNA association. Nat Commun. 2017;8:14011. https://doi.org/10.1038/ncomms14011. (Epub 2017/01/30).
Hallett ST, Campbell Harry I, Schellenberger P, Zhou L, Cronin NB, Baxter J, et al. Cryo-EM structure of the Smc5/6 holo-complex. Nucleic Acids Res. 2022. https://doi.org/10.1093/nar/gkac692. (Epub 20220822).
Adamus M, Lelkes E, Potesil D, Ganji SR, Kolesar P, Zabrady K, et al. Molecular insights into the architecture of the human SMC5/6 complex. J Mol Biol. 2020;432(13):3820–37. https://doi.org/10.1016/j.jmb.2020.04.024.
Yu Y, Li S, Ser Z, Kuang H, Than T, Guan D, et al. Cryo-EM structure of DNA-bound Smc5/6 reveals DNA clamping enabled by multi-subunit conformational changes. Proc Natl Acad Sci USA. 2022;119(23): e2202799119. https://doi.org/10.1073/pnas.2202799119. (Epub 20220601).
Ganji M, Shaltiel IA, Bisht S, Kim E, Kalichava A, Haering CH, et al. Real-time imaging of DNA loop extrusion by condensin. Science. 2018;360(6384):102–5. https://doi.org/10.1126/science.aar7831. (Epub 2018/02/22).
Davidson IF, Bauer B, Goetz D, Tang W, Wutz G, Peters JM. DNA loop extrusion by human cohesin. Science. 2019;366(6471):1338–45. https://doi.org/10.1126/science.aaz3418. (Epub 2019/11/21).
Wang XD, Hughes AC, Brandao HB, Walker B, Lierz C, Cochran JC, et al. In vivo evidence for ATPase-dependent DNA translocation by the Bacillus subtilis SMC condensin complex. Mol Cell. 2018;71(5):841–7. https://doi.org/10.1016/j.molcel.2018.07.006.
Pradhan B, Kanno K, Igarashi MU, Baaske MD, Wong JSK, Jeppsson K, et al. The Smc5/6 complex is a DNA loop extruding motor. bioRxiv. 2022. https://doi.org/10.1101/2022.05.13.491800.
Zabrady K, Adamus M, Vondrova L, Liao C, Skoupilova H, Novakova M, et al. Chromatin association of the SMC5/6 complex is dependent on binding of its NSE3 subunit to DNA. Nucleic Acids Res. 2016;44(3):1064–79. https://doi.org/10.1093/nar/gkv1021.
Piazza I, Rutkowska A, Ori A, Walczak M, Metz J, Pelechano V, et al. Association of condensin with chromosomes depends on DNA binding by its HEAT-repeat subunits. Nat Struct Mol Biol. 2014;21(6):560–8. https://doi.org/10.1038/nsmb.2831. (Epub 20140518).
Toselli-Mollereau E, Robellet X, Fauque L, Lemaire S, Schiklenk C, Klein C, et al. Nucleosome eviction in mitosis assists condensin loading and chromosome condensation. EMBO J. 2016;35(14):1565–81. https://doi.org/10.15252/embj.201592849. (Epub 2016/06/06).
Shaltiel IA, Datta S, Lecomte L, Hassler M, Kschonsak M, Bravo S, et al. A hold-and-feed mechanism drives directional DNA loop extrusion by condensin. Science. 2022;376(6597):1087–94. https://doi.org/10.1126/science.abm4012. (Epub 20220602).
Shi ZB, Gao HS, Bai XC, Yu HT. Cryo-EM structure of the human cohesin-NIPBL-DNA complex. Science. 2020;368(6498):1454. https://doi.org/10.1126/science.abb0981.
Bürmann F, Funke LFH, Chin JW, Löwe J. Cryo-EM structure of MukBEF reveals DNA loop entrapment at chromosomal unloading sites. Mol Cell. 2021;81(23):4891-906.e8. https://doi.org/10.1016/j.molcel.2021.10.011. (Epub 20211104).
Lopez-Serra L, Kelly G, Patel H, Stewart A, Uhlmann F. The Scc2-Scc4 complex acts in sister chromatid cohesion and transcriptional regulation by maintaining nucleosome-free regions. Nat Genet. 2014;46(10):1147–51. https://doi.org/10.1038/ng.3080.
Munoz S, Minamino M, Casas-Delucchi CS, Patel H, Uhlmann F. A role for chromatin remodeling in cohesin loading onto chromosomes. Mol Cell. 2019;74(4):664. https://doi.org/10.1016/j.molcel.2019.02.027.
Munoz S, Passarelli F, Uhlmann F. Conserved roles of chromatin remodellers in cohesin loading onto chromatin. Curr Genet. 2020;66(5):951–6. https://doi.org/10.1007/s00294-020-01075-x.
Roguev A, Wiren M, Weissman JS, Krogan NJ. High-throughput genetic interaction mapping in the fission yeast Schizosaccharomyces pombe. Nat Methods. 2007;4(10):861–6. https://doi.org/10.1038/nmeth1098. (Epub 2007/09/23).
Kim DU, Hayles J, Kim D, Wood V, Park HO, Won M, et al. Analysis of a genome-wide set of gene deletions in the fission yeast Schizosaccharomyces pombe. Nat Biotechnol. 2010;28(6):617–23. https://doi.org/10.1038/nbt.1628. (Epub 2010/05/16).
Wagih O, Usaj M, Baryshnikova A, VanderSluis B, Kuzmin E, Costanzo M, et al. SGAtools: one-stop analysis and visualization of array-based genetic interaction screens. Nucleic Acids Res. 2013;41(Web Server issue):W591–6. https://doi.org/10.1093/nar/gkt400. (Epub 2013/05/15).
Shannon P, Markiel A, Ozier O, Baliga NS, Wang JT, Ramage D, et al. Cytoscape: a software environment for integrated models of biomolecular interaction networks. Genome Res. 2003;13(11):2498–504. https://doi.org/10.1101/gr.1239303.
Palecek JJ. SMC5/6: multifunctional player in replication. Genes. 2019;10(1):E7. https://doi.org/10.3390/genes10010007.
Aragon L. The Smc5/6 complex: new and old functions of the enigmatic long-distance relative. In: Bonini NM, editor. Annual review of genetics, vol. 52. San Mateo: Palo Alto: Annual Reviews; 2018. p. 89–107. https://doi.org/10.1146/annurev-genet-120417-031353.
Lee KM, Nizza S, Hayes T, Bass KL, Irmisch A, Murray JM, et al. Brc1-mediated rescue of Smc5/6 deficiency: requirement for multiple nucleases and a novel Rad18 function. Genetics. 2007;175(4):1585–95. https://doi.org/10.1534/genetics.106.067801.
Lehmann AR, Walicka M, Griffiths DJF, Murray JM, Watts FZ, McCready S, et al. The rad18 gene of Schizosaccharomyces pombe defines a new subgroup of the SMC superfamily involved in DNA repair. Mol Cell Biol. 1995;15:7067–80. https://doi.org/10.1128/MCB.15.12.7067.
Morikawa H, Morishita T, Kawane S, Iwasaki H, Carr AM, Shinagawa H. Rad62 protein functionally and physically associates with the smc5/smc6 protein complex and is required for chromosome integrity and recombination repair in fission yeast. Mol Cell Biol. 2004;24(21):9401–13. https://doi.org/10.1128/MCB.24.21.9401-9413.2004.
Dixon SJ, Fedyshyn Y, Koh JLY, Prasad TSK, Chahwan C, Chua G, et al. Significant conservation of synthetic lethal genetic interaction networks between distantly related eukaryotes. Proc Natl Acad Sci USA. 2008;105(43):16653–8. https://doi.org/10.1073/pnas.0806261105.
Ryan CJ, Roguev A, Patrick K, Xu J, Jahari H, Tong Z, et al. Hierarchical modularity and the evolution of genetic interactomes across species. Mol Cell. 2012;46(5):691–704. https://doi.org/10.1016/j.molcel.2012.05.028.
Pebernard S, McDonald WH, Pavlova Y, Yates JR, Boddy MN. Nse1, Nse2, and a novel subunit of the Smc5-Smc6 complex, Nse3, play a crucial role in meiosis. Mol Biol Cell. 2004;15(11):4866–76. https://doi.org/10.1091/mbc.E04-05-0436.
Helmlinger D, Marguerat S, Villén J, Swaney DL, Gygi SP, Bähler J, et al. Tra1 has specific regulatory roles, rather than global functions, within the SAGA co-activator complex. EMBO J. 2011;30(14):2843–52. https://doi.org/10.1038/emboj.2011.181. (Epub 2011/06/03).
Verkade HM, Bugg SJ, Lindsay HD, Carr AM, O’Connell MJ. Rad18 is required for DNA repair and checkpoint responses in fission yeast. Mol Biol Cell. 1999;10(9):2905–18. https://doi.org/10.1091/mbc.10.9.2905.
Hudson JJR, Bednarova K, Kozakova L, Liao CY, Guerineau M, Colnaghi R, et al. Interactions between the Nse3 and Nse4 components of the SMC5-6 complex identify evolutionarily conserved interactions between MAGE and EID families. PLoS ONE. 2011;6(2):14. https://doi.org/10.1371/journal.pone.0017270.
Duan X, Sarangi P, Liu X, Rangi GK, Zhao X, Ye H. Structural and functional insights into the roles of the Mms21 subunit of the Smc5/6 complex. Mol Cell. 2009;35(5):657–68. https://doi.org/10.1016/j.molcel.2009.06.032.
Clouaire T, Rocher V, Lashgari A, Arnould C, Aguirrebengoa M, Biernacka A, et al. Comprehensive mapping of histone modifications at DNA double-strand breaks deciphers repair pathway chromatin signatures. Mol Cell. 2018;72(2):250-62.e6. https://doi.org/10.1016/j.molcel.2018.08.020. (Epub 2018/09/27).
Deshpande GP, Hayles J, Hoe KL, Kim DU, Park HO, Hartsuiker E. Screening a genome-wide S. pombe deletion library identifies novel genes and pathways involved in genome stability maintenance. DNA Repair. 2009;8(5):672–9. https://doi.org/10.1016/j.dnarep.2009.01.016. (Epub 2009/03/04).
Pan X, Lei B, Zhou N, Feng B, Yao W, Zhao X, et al. Identification of novel genes involved in DNA damage response by screening a genome-wide Schizosaccharomyces pombe deletion library. BMC Genomics. 2012;13:662. https://doi.org/10.1186/1471-2164-13-662. (Epub 2012/11/23).
Helmlinger D, Marguerat S, Villén J, Gygi SP, Bähler J, Winston F. The S. pombe SAGA complex controls the switch from proliferation to sexual differentiation through the opposing roles of its subunits Gcn5 and Spt8. Genes Dev. 2008;22(22):3184–95. https://doi.org/10.1101/gad.1719908.
Oravcová M, Gadaleta MC, Nie M, Reubens MC, Limbo O, Russell P, et al. Brc1 promotes the focal accumulation and SUMO ligase activity of Smc5-Smc6 during replication stress. Mol Cell Biol. 2018. https://doi.org/10.1128/MCB.00271-18. (Epub 2018/10/22).
Oravcová M, Boddy MN. Recruitment, loading, and activation of the Smc5-Smc6 SUMO ligase. Curr Genet. 2019;65(3):669–76. https://doi.org/10.1007/s00294-018-0922-9. (Epub 2019/01/02).
Pebernard S, Schaffer L, Campbell D, Head SR, Boddy MN. Localization of Smc5/6 to centromeres and telomeres requires heterochromatin and SUMO, respectively. EMBO J. 2008;27(22):3011–23. https://doi.org/10.1038/emboj.2008.220.
Lindroos HB, Strom L, Itoh T, Katou Y, Shirahige K, Sjogren C. Chromosomal association of the Smc5/6 complex reveals that it functions in differently regulated pathways. Mol Cell. 2006;22(6):755–67. https://doi.org/10.1016/j.molcel.2006.05.014.
Irmisch A, Ampatzidou E, Mizuno K, O’Connell MJ, Murray JM. Smc5/6 maintains stalled replication forks in a recombination-competent conformation. EMBO J. 2009;28(2):144–55. https://doi.org/10.1038/emboj.2008.273. (Epub 2009/01/23).
Peng XP, Lim S, Li SB, Marjavaara L, Chabes A, Zhao XL. Acute Smc5/6 depletion reveals its primary role in rDNA replication by restraining recombination at fork pausing sites. PLoS Genet. 2018;14(1):20. https://doi.org/10.1371/journal.pgen.1007129.
Torres-Rosell J, Machin F, Farmer S, Jarmuz A, Eydmann T, Dalgaard JZ, et al. SMC5 and SMC6 genes are required for the segregation of repetitive chromosome regions. Nat Cell Biol. 2005;7(4):412–9. https://doi.org/10.1038/ncb1239.
Torres-Rosell J, Sunjevaric I, De Piccoli G, Sacher M, Eckert-Boulet N, Reid R, et al. The Smc5-Smc6 complex and SUMO modification of Rad52 regulates recombinational repair at the ribosomal gene locus. Nat Cell Biol. 2007;9(8):923–31. https://doi.org/10.1038/ncb1619.
González-Medina A, Hidalgo E, Ayté J. Gcn5-mediated acetylation at MBF-regulated promoters induces the G1/S transcriptional wave. Nucleic Acids Res. 2019;47(16):8439–51. https://doi.org/10.1093/nar/gkz561.
Nugent RL, Johnsson A, Fleharty B, Gogol M, Xue-Franzén Y, Seidel C, et al. Expression profiling of S. pombe acetyltransferase mutants identifies redundant pathways of gene regulation. BMC Genomics. 2010;11:59. https://doi.org/10.1186/1471-2164-11-59. (Epub 20100122).
Elías-Villalobos A, Toullec D, Faux C, Séveno M, Helmlinger D. Chaperone-mediated ordered assembly of the SAGA and NuA4 transcription co-activator complexes in yeast. Nat Commun. 2019;10(1):5237. https://doi.org/10.1038/s41467-019-13243-w. (Epub 2019/11/20).
Lai J, Jiang J, Wu Q, Mao N, Han D, Hu H, et al. The transcriptional coactivator ADA2b recruits a structural maintenance protein to double-strand breaks during DNA repair in plants. Plant Physiol. 2018. https://doi.org/10.1104/pp.18.00123. (Epub 2018/02/20).
Jiang J, Ou X, Han D, He Z, Liu S, Mao N, et al. A diRNA-protein scaffold module mediates SMC5/6 recruitment in plant DNA repair. Plant Cell. 2022. https://doi.org/10.1093/plcell/koac191. (Epub 20220701).
Chiolo I, Minoda A, Colmenares SU, Polyzos A, Costes SV, Karpen GH. Double-strand breaks in heterochromatin move outside of a dynamic HP1a domain to complete recombinational repair. Cell. 2011;144(5):732–44. https://doi.org/10.1016/j.cell.2011.02.012. (Epub 2011 Feb 25).
Williams JS, Williams RS, Dovey CL, Guenther G, Tainer JA, Russell P. gammaH2A binds Brc1 to maintain genome integrity during S-phase. EMBO J. 2010;29(6):1136–48. https://doi.org/10.1038/emboj.2009.413
Moreno S, Klar A, Nurse P. Molecular genetic analysis of fission yeast Schizosaccharomyces pombe. Methods Enzymol. 1991;194:795–823. https://doi.org/10.1016/0076-6879(91)94059-l.
Maere S, Heymans K, Kuiper M. BiNGO: a Cytoscape plugin to assess overrepresentation of gene ontology categories in biological networks. Bioinformatics. 2005;21(16):3448–9. https://doi.org/10.1093/bioinformatics/bti551. (Epub 2005/06/24).
Lock A, Rutherford K, Harris MA, Hayles J, Oliver SG, Bähler J, et al. PomBase 2018: user-driven reimplementation of the fission yeast database provides rapid and intuitive access to diverse, interconnected information. Nucleic Acids Res. 2019;47(D1):D821–7. https://doi.org/10.1093/nar/gky961.
Paleček JJ, Vondrová L, Zábrady K, Otočka J. Multicomponent yeast two-hybrid system: applications to study protein-protein interactions in SMC complexes. Methods Mol Biol. 2019;2004:79–90. https://doi.org/10.1007/978-1-4939-9520-2_7.
Sergeant J, Taylor E, Palecek J, Fousteri M, Andrews E, Sweeney S, et al. Composition and architecture of the Schizosaccharomyces pombe Rad18 (Smc5-6) complex. Mol Cell Biol. 2005;25(1):172–84. https://doi.org/10.1128/MCB.25.1.172-184.2005.
Palecek J, Vidot S, Feng M, Doherty AJ, Lehmann AR. The SMC5-6 DNA repair complex: bridging of the SMC5-6 heads by the Kleisin, NSE4, and non-Kleisin subunits. J Biol Chem. 2006;281:36952–9. https://doi.org/10.1074/jbc.M608004200.
Varadi M, Anyango S, Deshpande M, Nair S, Natassia C, Yordanova G, et al. AlphaFold protein structure database: massively expanding the structural coverage of protein-sequence space with high-accuracy models. Nucleic Acids Res. 2022;50(D1):D439–44. https://doi.org/10.1093/nar/gkab1061.
Mirdita M, Schütze K, Moriwaki Y, Heo L, Ovchinnikov S, Steinegger M. ColabFold: making protein folding accessible to all. Nat Methods. 2022;19(6):679–82. https://doi.org/10.1038/s41592-022-01488-1. (Epub 20220530).
Byska J, Jurcik A, Furmanova K, Kozlikova B, Palecek JJ. Visual analysis of protein–protein interaction docking models using COZOID tool. Methods Mol Biol. 2020;2074:81–94. https://doi.org/10.1007/978-1-4939-9873-9_7. (Epub 2019/10/05).
Wood V, Gwilliam R, Rajandream MA, Lyne M, Lyne R, Stewart A, et al. The genome sequence of Schizosaccharomyces pombe. Nature. 2002;415(6874):871–80. https://doi.org/10.1038/nature724.
Kim D, Langmead B, Salzberg SL. HISAT: a fast spliced aligner with low memory requirements. Nat Methods. 2015;12(4):357–60. https://doi.org/10.1038/nmeth.3317. (Epub 20150309).
Li H, Handsaker B, Wysoker A, Fennell T, Ruan J, Homer N, et al. The sequence alignment/map format and SAMtools. Bioinformatics. 2009;25(16):2078–9. https://doi.org/10.1093/bioinformatics/btp352. (Epub 20090608).
Bonfield JK, Marshall J, Danecek P, Li H, Ohan V, Whitwham A, et al. HTSlib: C library for reading/writing high-throughput sequencing data. Gigascience. 2021. https://doi.org/10.1093/gigascience/giab007.
Ramírez F, Ryan DP, Grüning B, Bhardwaj V, Kilpert F, Richter AS, et al. deepTools2: a next generation web server for deep-sequencing data analysis. Nucleic Acids Res. 2016;44(W1):W160–5. https://doi.org/10.1093/nar/gkw257. (Epub 20160413).
Wang H, Dienemann C, Stützer A, Urlaub H, Cheung ACM, Cramer P. Structure of the transcription coactivator SAGA. Nature. 2020;577(7792):717–20. https://doi.org/10.1038/s41586-020-1933-5. (Epub 20200122).
We thank N. J. Krogan and M. N. Boddy for providing the yeast strains. We are grateful to C. Haering for his help with the Rotor HDA robot and M. Adamus for the critical reading of our manuscript.
Funding from the Ministry of Education, Youth and Sports of the Czech Republic (project INTER-COST LTC20033 to JJP) is gratefully acknowledged. BŠ and PK were supported by the Masaryk University Grants MUNI/R/1142/2021 and MUNI/R/1262/2022, respectively. MP, AM and JP were supported by the Charles University Grant PRIMUS/MED/26. We duly acknowledge the assistance of the GeneCore facility (EMBL Heidelberg) and Genomics CF (CEITEC; project LM2018132 funded by MEYS CR) with the NGS part of our project. The funders had no role in study design, data collection and analysis, decision to publish or preparation of the manuscript.
Ethics approval and consent to participate
Consent for publication
The authors declare no competing interests.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
About this article
Cite this article
Mahrik, L., Stefanovie, B., Maresova, A. et al. The SAGA histone acetyltransferase module targets SMC5/6 to specific genes. Epigenetics & Chromatin 16, 6 (2023). https://doi.org/10.1186/s13072-023-00480-z