PRDM9 activity depends on HELLS and promotes local 5-hydroxymethylcytosine enrichment

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Version of Record published: October 30, 2020 (This version)
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Accepted: September 16, 2020
Received: March 20, 2020

1. Of interest
Foxp3 depends on Ikaros for control of regulatory T cell gene expression and function

Rajan M Thomas, Matthew C Pahl ... Andrew D Wells

Research Article Apr 24, 2024
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Abstract

Meiotic recombination starts with the formation of DNA double-strand breaks (DSBs) at specific genomic locations that correspond to PRDM9-binding sites. The molecular steps occurring from PRDM9 binding to DSB formation are unknown. Using proteomic approaches to find PRDM9 partners, we identified HELLS, a member of the SNF2-like family of chromatin remodelers. Upon functional analyses during mouse male meiosis, we demonstrated that HELLS is required for PRDM9 binding and DSB activity at PRDM9 sites. However, HELLS is not required for DSB activity at PRDM9-independent sites. HELLS is also essential for 5-hydroxymethylcytosine (5hmC) enrichment at PRDM9 sites. Analyses of 5hmC in mice deficient for SPO11, which catalyzes DSB formation, and in PRDM9 methyltransferase deficient mice reveal that 5hmC is triggered at DSB-prone sites upon PRDM9 binding and histone modification, but independent of DSB activity. These findings highlight the complex regulation of the chromatin and epigenetic environments at PRDM9-specified hotspots.

Introduction

In sexual reproduction, genetic information from both parental genomes is reassorted through chromosome segregation during meiosis. Additional genetic diversity is generated by recombination events between parental homologous chromosomes (homologs) that take place during the first meiotic prophase. Meiotic recombination leads to reciprocal (crossover) and non-reciprocal (gene conversion) transfer of genetic information. Crossovers establish physical links between homologs that are maintained until the end of prophase of the first meiotic division and are essential for the proper segregation of homologs at the first meiotic division. Gene conversion without crossovers promotes interactions between homologs, thus mechanistically contributing to the proper execution of the crossover pathway. Gene conversion also leads locally to the replacement of small regions (typically, from a few to a few hundred base pairs) from one parental genome to the other (Chen et al., 2007). Therefore, meiotic homologous recombination enhances genetic diversity (Coop and Przeworski, 2007) and is essential for fertility (Hunter, 2015). Homologous recombination events are generated by the programmed induction of DNA double- strand breaks (DSBs) followed by their repair, as a crossover or not, with a chromatid from the homolog (Baudat and de Massy, 2007). Meiotic DSBs are tightly controlled in time, space, and frequency to drive the homologous recombination pathway while keeping genome integrity (de Massy, 2013; Keeney et al., 2014; Sasaki et al., 2010).

Remarkably, two distinct pathways control DSB localization (Lichten and de Massy, 2011). In several species, including plants and fungi, DSBs occur at promoter regions or regions of accessible chromatin without detectable sequence specificity. This pattern of DSB localization has been thoroughly analyzed in Saccharomyces cerevisiae (Pan et al., 2011). The DSB machinery, which involves several proteins including Spo11 that carries the catalytic activity for DNA cleavage (de Massy, 2013), is somehow directed to such accessible chromatin sites. Several factors that act locally, such as chromatin structure, but also higher order chromosome organization features are important for DSB formation at these accessible regions (Lam and Keeney, 2015). In contrast, in humans and mice, and possibly in some non-mammalian species (Baker et al., 2017), DSBs occur at sites bound by PRDM9 and not at promoters (Pratto et al., 2014; Smagulova et al., 2011). The Prdm9 gene, which is present in a wide range of metazoans, is expressed specifically in meiocytes, at the stage of meiotic DSB formation. It encodes a protein that has a sequence-specific DNA- binding domain with multiple potential targets in the genome. PRDM9 also has a PR-SET domain with methyltransferase activity and promotes the tri-methylation of lysine 4 (H3K4me3) and of lysine 36 (H3K36me3) of histone H3 on nucleosomes adjacent to PRDM9-binding sites (Grey et al., 2018). This methyltransferase activity is essential for DSB formation at PRDM9 sites (Diagouraga et al., 2018). In mice lacking PRDM9, DSBs form at promoters and enhancers (Brick et al., 2012; Mihola et al., 2019).

The various steps that take place from PRDM9 binding to DSB formation are still poorly understood. Specifically, it is not known how the DSB machinery is recruited or activated, and how the different molecular steps proceed in a local chromatin environment that is a priori not specified before PRDM9 binding. Moreover, upon binding, PRDM9 promotes chromatin modifications with the deposition of H3K4me3 and H3K36me3 on adjacent nucleosomes (Baker et al., 2014; Grey et al., 2017; Powers et al., 2016). One or both of these modifications are predicted to be required for DSB activity, because PRDM9 methyltransferase is essential for DSB activity at PRDM9 sites (Diagouraga et al., 2018), unless another substrate of PRDM9 methyltransferase is involved. In addition, these histone modifications may play a role in DSB repair. Indeed, ZCWPW1, a protein reader of H3K4me3 and H3K36me3, is required for efficient DSB repair (Huang et al., 2020; Li et al., 2019; Mahgoub et al., 2020; Wells et al., 2019). Whatever their exact role, the presence of both histone modifications leads to a unique chromatin landscape at PRDM9 sites that is not present at promoters, where H3K36me3 is depleted (Grey et al., 2017; Lam et al., 2019; Powers et al., 2016). Therefore, the specific chromatin environment at PRDM9 sites may be important for DSB activity and repair. In mice lacking PRDM9, where DSBs form mainly at promoters and enhancers, an inefficient DSB repair is observed (Brick et al., 2012; Hayashi and Matsui, 2006), which could be due to the chromatin environment at those sites, and/or alternatively to improper regulation of DSB formation.

Other histone modifications have been identified at PRDM9 sites (Buard et al., 2009; Davies et al., 2016; Lam et al., 2019). It has been proposed that epigenetic features at DSB hotspots are also responsible for some of the observed DSB activity differences in male and female mouse meiosis (Brick et al., 2018). Indeed, besides chromatin, the global cytosine methylation level is different between sexes: low in prophase oocytes (Kagiwada et al., 2013; Seisenberger et al., 2012) and high in spermatocytes (Gaysinskaya et al., 2018). Cytosine methylation is a dynamic epigenetic modification that can be removed by the actions of ten-eleven-translocation (TET) enzymes, the first product of which is 5-hydroxymethylcytosine (5hmC) (Tahiliani et al., 2009). Interestingly, a local increase in 5hmC has been detected at PRDM9 sites in mouse spermatocytes (Brick et al., 2018), indicative of another potential layer of modification at DSB sites.

To gain insights into these molecular steps and to identify proteins involved at PRDM9-binding sites, we developed a proteomic approach to identify PRDM9 partners. We found that HELLS, a member of the SNF2-like family of chromatin remodelers, interacts with PRDM9. This interaction has also been recently shown by Spruce and colleagues (Spruce et al., 2020). Interestingly, HELLS was previously implicated in the regulation of DNA methylation, transposable element expression, heterochromatin dynamics, and DSB repair in somatic cells (Burrage et al., 2012; Dennis et al., 2001; Kollárovič et al., 2020; Lungu et al., 2015; Yu et al., 2014b). HELLS is also required for female and male meiosis (De La Fuente et al., 2006; Zeng et al., 2011). A recent study showed that HELLS is needed for proper meiotic DSB localization and acts as a PRDM9-dependent chromatin remodeler of meiotic hotspots (Spruce et al., 2020). Here, we found that in mouse male meiosis, HELLS is directly involved in the control of DSB activity by ensuring PRDM9 binding and thus DSB formation at PRDM9-dependent sites, consistent with the results obtained by Spruce et al., 2020. This HELLS activity appears to solve the challenge of chromatin accessibility for PRDM9 binding. We also show that HELLS-dependent PRDM9 binding and PRDM9 methyltransferase activity are required for efficient 5hmC enrichment at PRDM9-binding sites. This epigenetic modification is a feature of PRDM9-specified hotspots that is not dependent on DSB formation.

Results

HELLS interacts with PRDM9

To identify proteins that interact with PRDM9 we first chose to express a tagged version of human PRDM9 in HeLa S3 cells, which do not express PRDM9 (Morin et al., 2008), and performed immunoprecipitation (IP) followed by mass spectrometry analysis allowing us to identify candidates that are not germline-specific. We generated two stable cell lines that express the human PRDM9^A allele (Baudat et al., 2010) with an epitope tag (FLAG-HA) inserted at the amino- (Nt) or carboxy-terminal (Ct) end (see Materials and methods). Unmodified HeLa S3 cells were used as negative control. We purified tagged PRDM9^A-containing complexes from HeLa S3 cell nuclear extracts by FLAG affinity, followed by HA affinity purification (Table 1—source data 1).

Table 1

HELLS is co-immunoprecipitated with PRDM9.

Two independent immunoprecipitation experiments were performed using HeLa cells and mouse testis extracts. In the first experiment, HeLa S3 cells that express N-terminally (Nter) or C-terminally (Cter) tagged human PRDM9 or without PRDM9 expression vector (no PRDM9) were used to identify proteins that interacts with PRDM9 after size selection (95–120 kD and 70–80 kD), and without size selection. Mouse testis extracts were prepared without (rep1) or after incubation with benzonase (rep2) (in duplicate). IP were performed with an anti-PRDM9 antibody or with normal rabbit serum (mock). For each protein (PRDM9 and HELLS), the total number of peptides, the protein rank in the whole set of proteins with at least one peptide, and ranked by number of peptides, and the sequence coverage are indicated; na: not applicable. For mouse testis extracts, the rank difference of the label free quantification intensity (LFQ) between IPs with anti-PRDM9 and mock are indicated. The full list of the identified peptides is in Supplementary file 1. Extracts analysis by electrophoresis are presented in Table 1—source data 1.

IP	Total peptides PRDM9	Rank PRDM9	Sequence coverage PRDM9 (%)	Total peptides HELLS	Rank HELLS	Sequence coverage HELLS (%)
HeLa with size selection
HeLa PRDM9 Nter 95–120 KD 70–80 KD	0 7	na 1/21	na 6.4	11 0	1/16 na	11.9 na
HeLa PRDM9 Cter 95–120 KD 70–80 KD	0 7	na 3/34	na 7.3	4 0	2/32 na	4.4 na
HeLa no PRDM9 95–120 KD 70–80 KD	0 0	na	na	0 0	na	na
HeLa without size selection
HeLa PRDM9 Nter	38	6/447	29.4	97	1/447	48.1
HeLa PRDM9 Cter	35	4/364	33.7	44	1/364	37.6
HeLa no PRDM9	0	na	na	0	na	na
Mouse testis rep1
IP PRDM9	24	27/571	35.1	14	75/571	24.1
mock	1	538/571	1.2	6	211/571	9.3
LFQ Rank difference		441			113
Mouse testis rep2 (+benzonase)
IP PRDM9	14 15	39/890 41/948	26.3	6 7	187/890 178/948	11
mock	1 0	782/890 na	1.4	5 1	323/890 506/948	7.2
LFQ Rank difference		870 688			122 468

Table 1—source data 1 Purification of protein complexes. (A) Western blot analysis after complex purification by Flag-HA of extracts from HeLa S3 cells. HeLa S3 cells without PRDM9 expression vector, or expressing human PRDM9 tagged with Flag-HA at the C-terminus (PRDM9-Ct) or N-terminus (PRDM9-Nt) were used. Protein fractions of the extracts before IP (S1: cytoplasmic fraction, S2: nuclear fraction as input for IPs, ppt: insoluble pellet) and after the affinity purification steps were analyzed by western blotting using an anti-PRDM9 antibody. (B) Analysis of affinity-purified proteins after silver staining (sample without size selection). Eluates 1, 2 and resin fractions obtained from affinity purification (HA) of extracts initially prepared from HeLa S3 cells without PRDM9 expression vector (M), or expressing human PRDM9 tagged with Flag-HA at the C-terminus (Ct) or at the N-terminus (Nt) were separated by electrophoresis and silver stained. Mixtures of Eluate 1 and 2 were used for mass spectrometry analysis. (C) Western blot analysis of complex purification using an anti-PRDM9 antibody and mouse testes extracts (Mouse testis rep1). Protein extracts obtained during the Dignam-based purification (S1: cytoplasmic fraction, S2: nuclear fraction, S3: DNase-treated, and ppt: pellet) were loaded. Input (S2), unbound (UB), and proteins immunoprecipitated (IP) with an anti-PRDM9 antibody or normal rabbit serum (mock) were analyzed by western blotting. Detection was with an anti-PRDM9 antibody. Loading: 1 and 10% of input and IP samples, respectively. (D) Analysis of affinity-purified proteins by silver staining (Mouse testis rep1). Input, and samples IP with an anti-PRDM9 antibody or with normal rabbit serum (mock) were loaded. Bovine serum albumin (BSA) was used as control. Proteins were separated by electrophoresis and silver stained. (E) Western blot analysis of complex purification using an anti-PRDM9 antibody in extracts from mouse testes incubated with benzonase (Mouse testis rep 2), in duplicate (a and b). Protein extracts obtained during the Dignam-based purification steps (S1: cytoplasmic fraction, S2: nuclear fraction, S3: DNase-treated, and ppt: pellet) were loaded. Input (S2) and proteins IP with an anti-PRDM9 antibody or rabbit serum (mock) were analyzed by western blotting. Detection was with an anti-PRDM9 antibody. Loading: 1% and 10% of input and IP samples. (F) Analysis of affinity purified proteins by silver staining (Mouse testis rep2). Input, and samples IP with an anti-PRDM9 antibody or with normal rabbit serum (mock) were loaded. BSA was used as control. Proteins were separated by electrophoresis and stained with silver.: https://cdn.elifesciences.org/articles/57117/elife-57117-table1-data1-v2.pdf
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First, we carried out pilot experiments by selecting proteins with a size that ranged between 70 and 80 kD and between 95 and 120 kD after silver staining to potentially identify PRDM9 and other proteins, respectively. PRDM9 peptides were the first and the third most abundant peptides for Nt- and Ct-tagged PRDM9, respectively, only in the 70–80 kD size range (Table 1). Although the predicted molecular weight (MW) of tagged PRDM9 is 103 kD, its detection in the 70–80 kD size range is compatible with its faster than predicted migration during denaturing gel electrophoresis (see western blots in Table 1—source data 1). HELLS peptides were the first and the second most abundant peptides for Nt- and Ct-tagged PRDM9, respectively, only in the 95–120 kD size range, in agreement with HELLS predicted MW (97 kD) (Jarvis et al., 1996). Then, we repeated the experiments, but without size selection and by analyzing the full protein content after affinity purification. This analysis confirmed the pilot experiment findings, and highlighted HELLS as a major PRDM9 partner. In this condition, with both Nt- and Ct-tagged PRDM9, HELLS was the first in the list of proteins identified by mass spectrometry and ranked by peptide abundance. We did not detect HELLS peptides in IP experiments from HeLa S3 cells without the PRDM9-expressing vector. The PRDM9 and HELLS peptide counts, and protein coverages are shown in Table 1 (see Supplementary file 1 for the full list of proteins). We did not perform any other analysis or quantification of the proteome present in these samples for this study.

As HELLS is expressed in gonads and is essential for gametogenesis (De La Fuente et al., 2006; Zeng et al., 2011), we then tried but failed to detect any interaction between HELLS and PRDM9 by western blotting after IP of mouse testis protein extracts. This could be due to technical problems linked to the used antibodies since this interaction was recently detected in mouse testis extracts by Spruce et al., 2020. Therefore, we used mass spectrometry after IP with a polyclonal antibody against PRDM9 or normal rabbit serum (mock) (Table 1, Table 1—source data 1). The relative abundance of HELLS peptides was lower in the assays with mouse testis extracts compared with HeLa S3 cell extracts, partly due to higher noise. Nevertheless, HELLS peptides were enriched in extracts purified with the anti-PRDM9 antibody, compared with mock control. In three independent experiments, 14, 6, and 7 HELLS peptides were obtained after IP with the anti-PRDM9 antibody, and 6, 5, and one in the mock controls (Table 1). HELLS enrichment in IP experiments with the anti-PRDM9 antibody was also revealed by quantification based on the Label-Free-Quantification ranks (Table 1 and Supplementary file 1).

As a complementary approach to proteomics, we searched for PRDM9 partners by yeast two-hybrid screening. Using mouse PRDM9 without zinc fingers as bait and a mouse juvenile testis cDNA bank, we identified six clones that corresponded to HELLS, indicating a direct interaction between PRDM9 and HELLS. All six clones shared a domain that included residues 30 to 448 of HELLS (Figure 1). To better map the HELLS region involved in the interaction with PRDM9, we generated different HELLS constructs and found that the C-terminal region (569-821) of HELLS was dispensable for this interaction (Figure 1B). We could not detect any interaction with PRDM9 upon deletions at the N-terminus or C-terminus of the 1–569 region, such as in the HELLS constructs 193–569 and 1–408, respectively. This suggests the potential involvement of the N-terminal (1-193) and of the central (408-569) regions of HELLS in the interaction with PRDM9 (Figure 1B and Figure 1—figure supplement 1).

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HELLS interacts with PRDM9.

(A) Domains of PRDM9 and HELLS PRDM9 includes a Krüppel-associated box domain (KRAB), a synovial sarcoma-X break point-repression domain (SSXRD), a Su(var)3–9, Polycomb-group protein enhancer of zeste and trithorax-group protein TRX domain (PR/SET) that is preceded and followed by zinc-finger domains (ZK and ZF, respectively), and a C2H2-type zinc-finger array (C2H2 ZF array). HELLS contains a coiled-coil domain, a helicase ATPase domain, and a helicase C-terminal domain. (B) Interaction between PRDM9 and HELLS by yeast two-hybrid assays. Full-length and four fragments of mouse HELLS were used to test for interaction with mouse PRDM9 (full length). HELLS domains were fused to the Gal4 activation domain (GAD), and PRDM9 was fused to the Gal4 DNA-binding domain (GBD). A positive interaction was detected for full-length HELLS and fragment 1–569. Growth was tested on medium without leucine and tryptophan (LW), without leucine, tryptophan and histidine (LWH), and without leucine, tryptophan and histidine with 5 mM amino-triazole (LWH + 5 mM AT). A diploid strain that expresses pGAD-REC114 and pGBD-MEI4 (Kumar et al., 2010) was used as positive control. The HELLS region of the cDNAs isolated by yeast two-hybrid screening is shown. Controls are shown in Figure 1—figure supplement 1.

HELLS is required for PRDM9-dependent meiotic DSB formation

To evaluate the functional role of HELLS in meiotic recombination, we generated a mouse line in which Hells was conditionally ablated only during male meiosis by meiotic-specific expression of CRE under the control of the Stra8 promoter on a transgene (Sadate-Ngatchou et al., 2008) (Hells cKO) (Figure 2—figure supplement 1), because HELLS is essential for mouse development (Geiman et al., 2001). A previous study where HELLS-deficient testes were analyzed by allografting embryonic tissues showed that HELLS is required for meiotic progression during spermatogenesis (Zeng et al., 2011). A potential interpretation for this meiotic defect was that alterations of DNA methylation in the absence of HELLS may affect, directly or indirectly, some properties of meiotic prophase and synapsis between homologous chromosomes (Zeng et al., 2011). This phenotype shares some similarity with the defects observed in Hells KO oocytes (defects in meiotic recombination and homologous synapsis, and changes in DNA methylation at repetitive DNA elements and pericentric heterochromatin) (De La Fuente et al., 2006).

Therefore, to test whether HELLS is directly implicated in meiotic recombination, we first precisely determined the meiotic stage(s) and steps that could be affected by HELLS depletion. In this study, we used various mouse strains with wild-type Hells alleles (Hells^fl/+, Hells^fl/+ Stra8-Cre^Tg, Hells^fl/-) that are all named Hells CTRL hereafter. Meiotic-specific Hells mutant mice were Hellsfl^fl/-Stra8-Cre^Tg and are named Hells cKO hereafter.

Western blot analysis of wild-type mouse testis whole cell extracts showed that HELLS protein could be detected from 4 days post-partum (dpp) to 15 dpp and in adults. PRDM9 was detected from nine dpp when cells have entered meiosis, but not at 4 and 6 dpp before meiosis entry (Figure 2—figure supplement 2). In testis nuclear extracts from 22 dpp Hells cKO animals, HELLS level was greatly reduced (Figure 2A), but not the nuclear PRDM9 protein level. The residual HELLS protein expression in testis nuclear extracts from Hells cKO mice might be due to incomplete CRE-induced deletion of Hells in some spermatocytes, as suggested by the cytological analysis presented below. We analyzed HELLS staining by immunofluorescence on spread spermatocytes of adult Hells CTRL and Hells cKO mice (Figure 2B). In Hells CTRL nuclei, we could detect HELLS as punctuate staining that covered nuclear chromatin, with the highest intensity at leptotene and zygotene and absence of specific staining at later stages (Figure 2—figure supplement 3). In Hells cKO nuclei, we did not detect HELLS staining in 75% of leptotene and zygotene nuclei, but could observe a weak HELLS staining in about 25% of nuclei (not shown). Thus, in some Hells cKO spermatocytes, HELLS expression was not completely abolished, and the protein was still present in the nucleus. Histological analysis of Hells cKO mice revealed spermatogenesis defects with 89% of tubules without haploid cells (Figure 2C,D), suggesting an arrest of spermatocyte differentiation. The presence of 11% of tubules with some haploid cells might be explained by incomplete HELLS depletion in some spermatocytes. Moreover, the percentage of tubules with one or more TUNEL-positive cells was increased, indicative of apoptotic cells undergoing massive genomic DNA breakage (Figure 2E and Figure 2—figure supplement 4).

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Meiotic prophase is defective in *Hells* cKO spermatocytes.

(A) Detection of PRDM9, HELLS and SYCP3 expression in nuclear fractions of testes from *Hells* CTRL (*Hells^fl/+* and *Hells^fl/-*) and *Hells* cKO mice at 22 dpp. Hells alleles are presented in Figure 2—figure supplement 1. HELLS and PRDM9 expression are presented in Figure 2—figure supplement 2. (B) Representative spreads of early zygotene spermatocyte nuclei from synchronized testes from *Hells* CTRL and *Hells* cKO mice after staining for DNA (DAPI, white or blue), SYCP3 (white or red) and HELLS (white or green) (top panels) or PRDM9 (white or green) (bottom panels). Anti-HELLS antibody from rabbit was used for these staining. Scale bar, 10 μm. HELLS and PRDM9 detection kinetics are presented in Figure 2—figure supplements 3 and 5. (C) Periodic acid-Schiff (PAS) staining of testis sections from 40 dpp *Hells* CTRL and *Hells* cKO mice. To visualize the glycoproteins/acrosomes (violet) and nuclei (blue), testis sections were stained with PAS and counterstained with hematoxylin. *Hells* CTRL testis sections (left panel) show normal spermatogenesis with well-organized stages of germ cell development, round spermatids with PAS-positive normal acrosomal caps, elongating and elongated spermatids. *Hells* cKO testis sections (right panel) show defective spermatogenesis with only few elongated spermatids (black arrow). Scale bar, 50 μm. (D) Proportions of seminiferous tubules without and with spermatids (mean ± SD) in testis sections from *Hells* CTRL and *Hells* cKO mice at 40 dpp. n = 4 testis sections from two mice. Data are available in Figure 2—source data 1. (E) Apoptosis detected by TUNEL assay in *Hells* CTRL and *Hells* cKO testes at 40 dpp. n = 2 testis sections from one mouse. TUNEL-positive cells are shown in Figure 2—figure supplement 4. Data are available in Figure 2—source data 1. (F) SYCP3 (red) and SYCP1 (green) staining of pachytene (*Hells* CTRL) and pachytene-like (*Hells* cKO) spermatocyte nuclei from 40 dpp mice. Arrowheads, unsynapsed chromosomes. White arrow, non-homologous synapsis. Blue arrows, sex chromosomes. Scale bar, 10 μm. (G) Representative spreads of early zygotene and pachytene or pachytene-like spermatocyte nuclei from 40 dpp *Hells* CTRL and *Hells* cKO mice, respectively, after staining for SYCP3 (white or red), DMC1 (white or green) and γH2AFX (white or blue). Scale bar, 10 μm.

Figure 2—source data 1 Quantification of spermatid and TUNEL-positive sections.: https://cdn.elifesciences.org/articles/57117/elife-57117-fig2-data1-v2.xlsx
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By immunostaining of spread spermatocytes, we showed that in Hells cKO mice, spermatocytes entered meiotic prophase and progressed until a pachytene-like stage with chromosomes only partially synapsed in most nuclei, whereas some nuclei had fully synapsed chromosomes (Figure 2F), consistent with previous observations on Hells-deficient spermatocytes (Zeng et al., 2011). We detected chromosome axes by the presence of the axial protein SYCP3, and synapses by the presence of the central element protein SYCP1. Ninety three percent of Hells CTRL nuclei that showed full-length axes were at the pachytene stage with 19 fully synapsed autosomes and a γH2AFX-positive chromatin domain containing the X and Y-chromosomes, called sex body. In contrast, only 13% of Hells cKO nuclei with full-length axes were similar to wild-type looking pachytene nuclei. This population of wild-type pachytene nuclei in Hells cKO mice could be due to incomplete depletion of HELLS in some spermatocytes, as discussed above.

Interestingly, in most Hells cKO spermatocytes, despite the normal level of nuclear PRDM9 detected by western blotting (Figure 2A), the PRDM9 signal detected by immunostaining was much reduced compared with wild-type (Figure 2B, Figure 2—figure supplement 5). As in nuclear spreads proteins that are not tightly bound to chromatin can be partially lost, this low PRDM9 signal in Hells cKO samples could indicate that in the absence of HELLS, PRDM9 localizes in the nucleus, but does not bind to chromatin efficiently. Overall, the DSB activity did not seem to be affected because we detected a large number of DMC1 foci. Conversely, DSB repair appeared to be defective, as indicated by the persistence of DMC1 and γH2AFX foci, and the absence of a normal XY sex body at the pachytene-like stage (Figure 2G).

To directly test DSB activity and localization in the absence of HELLS, we performed chromatin IP with an anti-DMC1 antibody followed by single-strand DNA sequencing (DMC1 ChIP-SSDS). DMC1 ChIP-SSDS allows recovering single-strand DNA bound by the strand exchange protein DMC1 (Khil et al., 2012). We performed these experiments in two wild-type (Hells CTRL) and two Hells cKO mice. Both wild-type and mutant mice express the PRDM9^Dom2 variant that binds to a specific set of genomic sites and promotes DSB formation at those sites (Brick et al., 2012; Grey et al., 2017). We detected 11133 and 17117 peaks of DMC1 enrichment in the Hells CTRL and Hells cKO samples, respectively. This indicated the presence of DSB activity in both genetic contexts, as observed by immunofluorescence. However, only 1129 peaks were common, representing 10% of Hells CTRL peaks, and 6.6% of Hells cKO peaks (Figure 3A, Figure 3—figure supplement 1). Analysis of the signal intensity in the genotype-specific peaks (Hells CTRL -specific and Hells cKO-specific) showed the absence of detectable signal in one genotype within peaks specific to the other genotype (Figure 3B). In the 1129 common peaks, the average DMC1 enrichment intensity was higher in Hells CTRL than in Hells cKO samples (Figure 3B). Among these common peaks, analysis of individual peak intensities revealed three subgroups, one subgroup with stronger intensity in Hells CTRL (n = 898 peaks), one subgroup with stronger intensity in Hells cKO (n = 154 peaks), and a smaller subgroup (n = 77 peaks) where the peak intensity was similar in both genotypes (Figure 3—figure supplement 2A). The group of 898 peaks with stronger intensity in Hells CTRL corresponded to DSB sites specified by PRDM9^Dom2. Indeed, an enrichment for H3K4me3 at these sites was observed specifically in the B6 strain that expresses PRDM9^Dom2, but not in the congenic RJ2 strain that expresses PRDM9^Cst, which binds to distinct genomic sites (Figure 3—figure supplement 2B). This suggests that these 898 peaks with stronger DMC1 intensity (in the cell population) in Hells CTRL may have a lower DSB level in Hells cKO, or may be active only in a smaller cell fraction in Hells cKO mice. We favor the second hypothesis, because our cytological analyses showed that HELLS is still detected in a small fraction of Hells cKO spermatocytes. The group of 154 peaks with higher DMC1 enrichment in Hells cKO were in regions with PRDM9-independent H3K4me3 enrichment (Figure 3—figure supplement 2B), suggesting a specific induction of DSB activity at these sites in the absence of HELLS. The group of 77 peaks with similar DMC1 intensity in Hells CTRL and Hells cKO showed a weak PRDM9-independent H3K4me3 enrichment. A low level of DSB activity at PRDM9-independent sites has been detected in mice that express PRDM9, and could account for these peaks (Smagulova et al., 2016).

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HELLS is required for the formation of meiotic DSBs at sites of PRDM9-dependent DSB formation; DSBs are directed at default sites in the absence of HELLS.

(A) Limited overlapping between DSB hotspots from *Hells* CTRL and *Hells* cKO testis samples. Only hotspot centers (DMC1-SSDS peaks) that overlapped within a 400bp-window were considered as common. The others were considered as *Hells* CTRL- or *Hells* cKO-specific hotspots. Controls are shown in Figure 3—figure supplement 1. (B) Distribution of the DMC1-SSDS signal from *Hells* CTRL and *Hells* cKO testis samples around *Hells* CTRL, *Hells* cKO and common hotspots (as defined in (A)). The heatmaps show the DMC1-SSDS normalized fragments per million, calculated in a −5 kb to +5 kb window around hotspot centers and averaged within 10bp-bins. For the *Hells* CTRL - or *Hells* cKO-specific hotspots, the sites on the heatmaps were ranked by decreasing DMC1 intensity (from top to bottom) in the genotype where the peaks were detected. For the common hotspots, the sites were ranked by decreasing DMC1 intensity (from top to bottom) in *Hells* CTRL mice. The averaged profiles represent the mean DMC1-SSDS signal for each group. The analysis of common hotspots is shown in Figure 3—figure supplement 2. (C) Wide overlapping of DSB hotspots from *Hells* cKO and *Prdm9* KO testis samples. Hotspot (DMC1-SSDS peaks) centers that overlapped within a 400bp-window were considered as common. The others were considered to be *Hells* cKO- or *Prdm9* KO-specific hotspots. *Prdm9* KO data were from GSE99921 (Brick et al., 2012). (D) The DMC1-SSDS signal in *Prdm9* KO testis samples is either *Prdm9* KO-specific (i.e. not overlapping) or overlapping with *Hells* cKO-specific hotspots (as defined in (C)). Density of hotspot number is plotted as a function of the DMC1 signal in *Prdm9* KO mice, expressed as FPMtype1 (type1-single-strand DNA fragments Per Million of mapped reads, see Materials and methods and Khil et al., 2012 for details). (E) DSB maps for *Hells* CTRL (blue) and *Hells* cKO (orange) testis samples (this study, two replicates for each genotype) and *Prdm9* KO testis samples (black, GSE99921; Brick et al., 2012) at a representative region of chromosome 1 (185.1Mb-185.5Mb). (F) Enrichment of PRDM9 and H3K4me3 is reduced at hotspots in *Hells* cKO compared with *Hells* CTRL samples. PRDM9 and H3K4me3 ChIP/Input ratios were calculated at several B6 (PRDM9^Dom2)-specific hotspots (*Pbx1a*, *14a*, A3, *17b*), at the *Sycp1* promoter (only for H3K4me3), and at two control regions that contain PRDM9^Cst-specific hotspots (*Psmb9.8* and *Hlx1.6*). All ratios were normalized to the ratios at *Hlx1.6*. At the four B6-specific hotspots, the difference between *Hells* cKO and *Hells* CTRL was statistically significant (two-tailed Mann-Whitney, p=0.0002). Data are available in Figure 3—source data 1.

Figure 3—source data 1 PRDM9 and H3K4me3 ChIP-qPCR.: https://cdn.elifesciences.org/articles/57117/elife-57117-fig3-data1-v2.xlsx
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To better understand the low overlap of DMC1 peaks in Hells CTRL and Hells cKO mice, we compared the Hells cKO peaks with those mapped in Prdm9 KO mice. When PRDM9 is defective (such as in Prdm9 KO mice) DSBs are formed at a different set of genomic sites, also called default sites. These sites overlap mainly with promoters and enhancers and are enriched in H3K4me3 (Brick et al., 2012). Remarkably, 85% of Hells cKO peaks overlapped with peaks detected in Prdm9 KO mice (Figure 3C and E). This demonstrated that in the absence of HELLS, DSBs are no longer formed at PRDM9 sites, but are induced at default sites, similarly to what observed in Prdm9 KO mice (Figure 3E). The lower number of peaks detected in Hells cKO samples (17117) compared with Prdm9 KO mice (27732) could be due to a lower signal in Hells cKO samples. We hypothesized that mainly low intensity peaks in Prdm9 KO mice should be undetectable in Hells cKO mice, and mainly high intensity peaks in Prdm9 KO should be detected in Hells cKO mice, thus contributing to the population of the 14543 overlapping peaks. Indeed, among the peaks mapped in Prdm9 KO samples, the peaks that were identified as overlapping with Hells cKO peaks were biased toward higher intensity compared with non-overlapping peaks (Figure 3D). The lower signal detected in Hells cKO could be explained by a difference in the sensitivity of the current ChIP-SSDS experiment and/or by a difference in DSB activity.

PRDM9-dependent DSB sites are characterized by several features that are implemented independently of DSB formation: PRDM9 binding, and enrichment for H3K4me3, H3K36me3 and H3K9ac on adjacent nucleosomes (Buard et al., 2009; Davies et al., 2016; Grey et al., 2017; Lam et al., 2019; Powers et al., 2016; Spruce et al., 2020). To identify the step of PRDM9-dependent DSB site designation affected by the absence of HELLS, we tested by ChIP-qPCR, PRDM9 binding and H3K4me3 levels at four representative PRDM9^Dom2 binding sites (Pbx1a, A3, 14a, 17b) that were used as reference in previous studies (Billings et al., 2013; Diagouraga et al., 2018). Enrichment for PRDM9 and for H3K4me3 were strongly reduced (at least by four-fold) at all four sites in Hells cKO spermatocytes compared with Hells CTRL cells (Figure 3F). This indicates that HELLS is required for efficient PRDM9 binding to its sites, consistent with the strong reduction in PRDM9 signal detected by immunofluorescence (Figure 2B). Moreover, this result provides a molecular interpretation for the absence of DSB activity at PRDM9-binding sites in Hells cKO spermatocytes.

HELLS and PRDM9 are required for 5hmC enrichment at meiotic hotspots

Recently, it was shown that HELLS interacts with all three TET methylcytosine dioxygenases (de Dieuleveult et al., 2020; Jia et al., 2017). Upon oxidation, the activity of TET enzymes on methylated cytosines (5mC) leads to a first product, 5-hydroxymethylcytosine (5hmC). It has been proposed that 5mC conversion to 5hmC allows regulating 5mC levels for proper gene expression (reviewed in Williams et al., 2012). Unlike 5mC, 5hmC is globally associated with euchromatin and is depleted on heterochromatin in somatic cells (Ficz et al., 2011). Interestingly, in mouse male germ cells, 5hmC is enriched at some enhancers and promoters (Gan et al., 2013; Hammoud et al., 2014), and at meiotic DSB hotspots in pachytene spermatocytes (Brick et al., 2018).

To test whether 5hmC enrichment was correlated with the DNA-binding specificity of PRDM9, we took advantage of two congenic mouse strains (B6 and RJ2) that express PRDM9 variants with distinct DNA-binding specificities (PRDM9^Dom2 and PRDM9^Cst, respectively). In both strains, the sites of PRDM9 binding and activity have been mapped, and localize to distinct sets of genomic sites (Grey et al., 2017). As the mapping of PRDM9-dependent DSB hotspots can be done with different molecular approaches (ChIP with anti-PRDM9, -H3K4me3, or -DMC1 antibodies), we used the DMC1 ChIP-SSDS data that provide the optimal specificity and sensitivity, as reference for hotspots (Grey et al., 2017). We performed the 5hmC analysis using genomic DNA isolated from 95% pure leptotene/zygotene cell populations (see Methods). In both B6 and RJ2 mouse strains, the 5hmC signal was correlated with DMC1 enrichment (Figure 4A and B), demonstrating that 5hmC enrichment depends on PRDM9 binding to its genomic targets.

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5hmC is enriched at PRDM9-dependent sites and correlates with PRDM9 occupancy.

(A) Average read enrichment and heatmaps showing 5hmC enrichment in the B6 (blue) and RJ2 (red) strains. Signal was calculated in a +/- 2 kb window around hotspot centers (determined by DMC1-SSDS). 5hmC enrichment was calculated from pooled replicates within 50bp bins and normalized by reads per million (RPM) and input. The sites on the heatmaps are ranked by decreasing DMC1-SSDS signal intensity from top to bottom. (B) Read distribution from DMC1 and 5hmC ChIP-seq experiments in the B6 (blue) and RJ2 (red) strains at representative DMC1 PRDM9^Dom2 (B6) and PRDM9^Cst (RJ2) specific sites on chromosome 1. Read distribution was calculated from pooled replicates within 50bp bins and normalized by library size and input, except for the DMC1 ChIP experiments. (C) Average read enrichment showing 5hmC enrichment (left y axis) and PRDM9 read enrichment (right y axis) in the B6 (blue) and RJ2 (red) strains centered in a +/- 2 kb window around DMC1 B6 and DMC1 RJ2 sites, respectively. Read distribution was calculated from pooled replicates within 50bp bins and normalized by library size and input. (D) 5hmC signal at hotspots is HELLS-dependent. Average read enrichment showing 5hmC in the B6 (blue) and *Hells* cKO (orange) strains centered in a +/- 2 kb window around the hotspot centers (DMC1-SSDS B6 sites). 5hmC enrichment was calculated from pooled replicates within 50bp bins and normalized by read per million (RPM) and input. (E) 5hmC signal at hotspots is dependent on PRDM9 methyltransferase activity. Average read enrichment showing 5hmC in the B6 (blue), RJ2 (red) and B6-Tg(YF)(magenta) strains centered in a +/- 2 kb window around the hotspot centers (DMC1-SSDS B6 and RJ2 sites). 5hmC enrichment was calculated from pooled replicates within 50bp bins and normalized by read per million (RPM) and input. (F) 5hmC signal at hotspots is independent of DSB formation. Average read enrichment showing 5hmC enrichment in the B6 (blue) and *Spo11* KO (green) strain centered in a +/- 2 kb window around the hotspot centers (DMC1-SSDS B6 sites). 5hmC enrichment was calculated form pooled replicates within 50bp bins and normalized by read per million (RPM) and input. The duplicate analysis for all genotypes is shown in Figure 4—figure supplement 2.

The heatmaps of 5hmC enrichment at DMC1 sites revealed a correlation between the strength of the DMC1 hotspots and that of 5hmC (Figure 4A). We obtained similar results when the heatmaps were generated based on sites defined by PRDM9 ChIP (Figure 4—figure supplement 1A). We also noted that the mean 5hmC signal at hotspots was higher in RJ2 than in B6 samples (Figure 4A, Figure 4—figure supplement 1A). This correlated with the greater occupancy of the PRDM9^Cst variant (expressed in RJ2 mice) compared with the PRDM9^Dom2 variant (expressed in B6 mice) (Grey et al., 2017). The 5hmC enrichment analysis and specifically the average enrichment plots showed a narrow distribution of the 5hmC enrichment that extended about +/- 250 bp from the peak center and overlapped closely with the enrichment profile of PRDM9 (Figure 4C). Peak centers were defined based on the DMC1 ChIP-SSDS signal and have been previously shown to overlap with PRDM9 DNA-binding motifs (Smagulova et al., 2011). However, 5hmC distribution was narrower than DMC1 distribution, which extends to the single-stranded DNA generated upon DSB end processing (Figure 4—figure supplement 1B). Moreover, the 5hmC maximum intensity was between the H3K4me3 peaks that delineate the positioned nucleosomes flanking the PRDM9 -binding sites (Baker et al., 2014; Figure 4—figure supplement 1B). Thus, 5hmC was predominantly taking place in the nucleosome-depleted region at and around PRDM9-binding sites.

Altogether, these findings suggest that 5hmC enrichment is functionally linked to PRDM9-binding activity. To directly test this hypothesis, we analyzed 5hmC in Hells cKO spermatocytes where PRDM9 binding to hotspots is defective (Figures 2B and 3F). Strikingly, 5hmC enrichment at hotspots was lost in Hells cKO spermatocytes (Figure 4D). This suggests that 5hmC enrichment at meiotic hotspots is promoted by HELLS and/or PRDM9 binding, or by one of the subsequent steps depending on HELLS and PRDM9. Therefore, we tested whether PRDM9 methyltransferase activity was required, using a mouse strain (named B6-Tg(YF)) where two PRDM9 variants of distinct DNA- binding specificities are produced: the PRDM9^Dom2 variant with wild-type methyltransferase activity, and the PRDM9^Cst-YF variant with defective methyltransferase activity due to a point mutation (Y357F) in the SET domain (Diagouraga et al., 2018; Wu et al., 2013). Our previous study established that the PRDM9^Cst-YF variant binds to the binding sites of PRDM9^Cst, but cannot catalyze the methylation of the surrounding histones (Diagouraga et al., 2018). In B6-Tg(YF) mice, 5hmC was enriched at the B6 DMC1 sites (bound by PRDM9^Dom2), as expected, but not at the RJ2 DMC1 sites bound by PRDM9^Cst-YF (Figure 4E). We conclude that PRDM9 binding is not sufficient and that its methyltransferase activity is also required for 5hmC enrichment. Then, to test whether 5hmC enrichment required also DSB activity (or downstream events), we analyzed 5hmC enrichment at hotspots in Spo11 KO mice in which DSB formation is defective. In these mice, 5hmC levels were identical to wild-type mice (Figure 4F). This result indicates that DSB formation is not required for 5hmC, and that a step between PRDM9 histone modification and DSB formation leads to 5hmC enrichment at meiotic hotspots.

We then analyzed the correlation of 5hmC enrichment with the strength of PRDM9, H3K4me3, SPO11-oligos and DMC1 enrichment. SPO11-oligos are the molecular intermediates generated after DSB formation by endonucleolytic cleavage of the strand to which SPO11 is covalently bound (Neale et al., 2005). SPO11-oligos data are available only for the B6 genotype (Lange et al., 2016). DMC1 enrichment reflects DSB formation, but is also influenced by features of DSB repair, and is not directly proportional to SPO11-oligos (Hinch et al., 2019). The correlation plots revealed that in the RJ2 strain, 5hmC was best correlated with PRDM9 and H3K4me3 enrichment, and in the B6 strain, with SPO11-oligo enrichment (Figure 4—figure supplement 1C). In both strains, the weakest correlation was between 5hmC and DMC1. This suggests that 5hmC enrichment at hotspots is better correlated with events directly linked to PRDM9 binding and DSB activity, rather than to DSB repair, which is consistent with the functional dependency reported above.

As 5hmC level at hotspots may depend on the density of CpG dinucleotides and of 5mC, it was important to examine the same correlations in function of the CpG content within hotspots (Figure 5—figure supplement 1A). Over a +/- 250 bp window around hotspot centers, the mean number of CpG was 4.4 (0.88 CpG/100b) in B6, and 4.3 (0.86 CpG/100b) in RJ2. Of note, the consensus motif for PRDM9^Dom2 and PRDM9^Cst does not include CpGs (Baker et al., 2015; Grey et al., 2017). The slight increase in CpG density around PRDM9^Dom2 hotspot was expected due to the process of GC-biased gene conversion (Duret and Galtier, 2009) that leads to higher GC content at meiotic recombination hotspots (Clément and Arndt, 2013; Grey et al., 2017). We then examined the methylation level at CpGs within +/- 250 bp from B6 and RJ2 hotspot centers that contained at least one CpG using published sodium bisulfite data from B6 samples (Gaysinskaya et al., 2018). As control, we analyzed the methylation level at four different types of genomic sites: (i) two families of transposable elements (LINE and IAP), and (ii) two sets of imprinted control regions (ICRs): one set methylated only in females (female-specific) and the other methylated only in males (male-specific). As shown before (Ferguson-Smith, 2011), we observed low cytosine methylation levels at female-specific ICRs and high methylation levels at male-specific ICRs and the transposable elements LINE and IAP (Figure 5—figure supplement 1B). Meiotic hotspots specific for each strain (B6 and RJ2) showed a similar median methylation level of at least 90% at all stages analyzed (B type spermatogonia, leptotene and pachytene spermatocytes), with a level comparable to what observed in the genome (Figure 5—figure supplement 1B). Note that B6 hotspots, but not RJ2 hotspots, were active in the strain where methylation was monitored. This suggests that overall, in the cell population, the level of hotspot methylation is high already before they are bound by PRDM9, with no further detectable local increase of cytosine modification upon PRDM9 binding. This property was also mentioned in a recent study where the methylation level at DSB sites was measured by Nucleosome Occupancy and Methylome sequencing (NOMe-seq) at different stages during spermatogenesis (Chen et al., 2020). As sodium bisulfite sequencing allows detecting both 5mC and 5hmC, we propose that the 5hmC enrichment we detected at active hotspots results from the conversion of pre-existing 5mC at these sites rather than de novo modification of unmodified cytosines.

We then evaluated the correlation between CpG content and 5hmC enrichment, by clustering hotspots according to their number of CpG dinucleotides within a region of +/- 250 bp around the center. We defined four groups of sites: (i) no CpG, (ii) 1–2 CpG, (iii) 3–5 CpG, and (iv)≥6 CpG dinucleotides. The average plots revealed that sites with higher numbers of CpGs tended to have higher 5hmC enrichment, in agreement with the fact that CpGs are the substrates for this modification (Figure 5A–B, Figure 5—figure supplement 1C). In contrast, the number of CpGs was not correlated with hotspot activity. This is shown by the overlapping curves of average plots for the four groups of CpG content of PRDM9, H3K4me3, and DMC1 enrichment (Figure 5—figure supplement 1D). Heatmaps within each group of hotspots with similar numbers of CpGs revealed also that for a given CpG content, the 5hmC level correlated with the PRDM9, H3K4me3, and DMC1 site intensity (Figure 5—figure supplement 1D), an observation coherent with the functional dependency on PRDM9 binding and methyltransferase activity reported above.

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5hmC enrichment at DSB sites sorted by CpG content and model.

(A) Average read enrichment and heatmaps showing 5hmC enrichment at DMC1-SSDS B6 sites. (B) Average read enrichment and heatmaps showing 5hmC enrichment at DMC1-SSDS RJ2 sites. In both panels, the signal was calculated in the B6 (blue) and RJ2 (red) strain in a +/- 2 kb window around the hotspot centers (determined by DMC1-SSDS) and sorted by CpG content with hotspots clustered in four groups: hotspots without CpGs, and three groups of similar size containing increasing numbers of CpGs (1–2, 3–5, and at least 6 CpGs). The number of sites for each group is indicated in the Methods section. For a given CpG content, the sites are ranked by decreasing DMC1-SSDS signal intensity from top to bottom. CpG content was calculated in a +/- 250 bp window around the hotspot centers. The same analysis but at PRDM9 sites is shown in Figure 5—figure supplement 1C. (C) Model for the targeting of DSB activity by PRDM9/HELLS in mouse male meiosis. (a) A potential PRDM9-binding site is a specific DNA motif in a region of chromatin with no specific feature. For each nucleosome, only two histone tails (H3) are shown. (b) The zinc-finger domain of PRDM9 (ZnF) interacts with specific DNA motifs. PRDM9 may be interacting as a complex with HELLS before binding to its target sites as suggested by Spruce et al., 2020. (c) HELLS promotes chromatin remodeling, enhancing accessibility of PRDM9 to its DNA motif and a stable interaction. (d) PRDM9 methyltransferase catalyzes H3K4me3 and H3K36me3 on adjacent nucleosomes. These histone modifications may or not be symmetric (Lange et al., 2016). H3K9Ac is also known to be enriched near PRDM9 -binding site at this stage (not shown). (e) Putative methylated cytosines (5mC) near the PRDM9-binding site are converted to 5hmC, suggesting the recruitment of a TET enzyme. (f) DSB forms at or adjacent to the PRDM9-binding site.

Discussion

A chromatin remodeler for PRDM9 binding

In 2010, the discovery that PRDM9 is the factor directing the location of meiotic DSBs in mammals raised several questions about the underlying molecular process. One of them was how the zinc- finger domain of PRDM9 gains access to its DNA-binding motifs. These DNA sites have no other reported function than being bound by PRDM9, and this occurs specifically in meiotic cells where Prdm9 is expressed. These sites are located throughout the genome, in genic and intergenic regions, and they do not appear to have any intrinsic feature beyond their DNA sequence. The only identified landmark is their higher GC content relative to their flanking regions that appears progressively over generations due to the process of GC-biased gene conversion during meiotic DSB repair at these sites (Clément and Arndt, 2013; Grey et al., 2017). Moreover, PRDM9-binding sites can differ between mouse strains because the PRDM9 DNA-binding domain is highly mutable, and multiple variants with distinct DNA-binding specificity are present in Mus musculus (Buard et al., 2014; Kono et al., 2014; Vara et al., 2019).

One of the major advances of this study, together with the parallel study from C. Baker’s group (Spruce et al., 2020), is the identification of the interaction between PRDM9 and HELLS, and the evidence of its essential role in allowing PRDM9 to access and stably bind to its binding sites (Figure 5C). The interaction between PRDM9 and HELLS was detected by IP-mass spectrometry and by yeast two-hybrid assays (this study) and by co-IPs (Spruce et al., 2020). In addition, and consistent with these interactions, ChIP experiments showed that HELLS is enriched at least at a fraction of PRDM9 sites, presumably the ones with the most efficient PRDM9 binding (Spruce et al., 2020). The chromatin configuration of PRDM9-binding sites has been analyzed by accessibility to MNase and to the transposase Tn5 (ATAC-seq). Before PRDM9 expression (in spermatogonia), most PRDM9-binding sites do not reveal specific accessibility compared with flanking genomic sequences (Chen et al., 2020). Conversely, when PRDM9 is expressed (leptonema), the binding sites show increased chromatin accessibility along few hundred base pairs on both sides of the PRDM9-binding site (Baker et al., 2014; Yamada et al., 2020). The footprint of PRDM9 binding is not detected by ATAC-seq, suggesting a short residency time (Spruce et al., 2020). As PRDM9 promotes H3K4me3 and H3K36me3 deposition on flanking nucleosomes, the chromatin organization at these sites can be examined and reveals a well-positioned arrangement of modified nucleosomes around PRDM9-binding sites. Overall, a striking change of chromatin configuration is observed upon PRDM9 binding, and HELLS plays an essential role in this process. This conclusion is based on the observation that in Hells cKO spermatocytes, PRDM9 binding (this study), PRDM9 dependent-H3K4me3 deposition, and chromatin accessibility (Spruce et al., 2020) cannot be detected at PRDM9-binding sites.

HELLS belongs to the SNF2-like family of chromatin remodelers (Flaus et al., 2006), but unlike other members of this family no ATP-dependent nucleosome remodeling activity could be detected in vitro (Burrage et al., 2012). However, in Xenopus laevis extracts, HELLS promotes nucleosome remodeling when forming a complex with CDCA7 that contains a 4-CXXC zinc-finger domain (Jenness et al., 2018). Therefore, it could be anticipated that in meiotic cells, HELLS is brought to PRDM9-binding sites by interacting with PRDM9. HELLS-dependent steps, such as nucleosome repositioning and/or stabilization and the subsequent opening of chromatin, could further stabilize the interaction of the PRDM9 zinc-finger domain with these sites, in a process partly similar to the one described for pioneer transcription factors (Mayran and Drouin, 2018). Functionally, HELLS absence leads to a phenotype comparable to the one observed upon Prdm9 genetic ablation. Indeed, in Hells cKO mice, meiotic DSB activity is undetectable at PRDM9 sites and is redirected to sites of open chromatin, such as promoters and enhancers (this study; Spruce et al., 2020), which are called default sites, like in Prdm9 KO mice (Brick et al., 2012). Therefore, HELLS is an essential determinant of meiotic DSB localization in mice.

Could HELLS have additional role(s) beyond promoting PRDM9 binding? As observed in Prdm9 KO mice, Hells cKO mice show a partial defect in DSB repair and homologous synapsis. By promoting nucleosome reorganization at PRDM9-binding sites, HELLS may contribute to DNA repair. This contribution may concern the chromatin of the broken and also the uncut chromatid because it has been proposed that PRDM9 binds not only to the chromatid where DSBs will occur but also to the intact template (Davies et al., 2016; Hinch et al., 2019). Such ‘symmetric binding’ might enhance interhomolog repair. In theory, HELLS activity could participate in DSB repair by regulating chromatin organization on the broken chromatid (for instance for strand resection), and on the uncut chromatid (for strand invasion). In support of this hypothesis, it has been shown that in somatic cells, HELLS is involved in and facilitates DSB repair (Burrage et al., 2012; Kollárovič et al., 2020). In somatic cells, HELLS might facilitate end-resection by interacting with and recruiting C-terminal interacting protein (CtIP) (Kollárovič et al., 2020). HELLS implication in genome integrity has also been detected in Neurospora crassa (Basenko et al., 2016) and Saccharomyces cerevisiae (Litwin et al., 2017). In S. cerevisiae, the HELLS orthologue Irc5 is required for DNA damage tolerance, and this function implies the loading of the cohesin complex at replication forks (Litwin et al., 2018). In S. cerevisiae, cohesin recruitment facilitates DSB repair (Ström et al., 2004; Unal et al., 2004). The hypothesis of a role for HELLS in meiotic DSB repair through enhancing end-resection and/or cohesin loading remains to be tested.

In other cellular contexts, HELLS is a major regulator of DNA methylation, specifically for the silencing of repeated DNA elements, and through the recruitment of the DNA methyltransferase DNMT3B (Myant and Stancheva, 2008; Zhu et al., 2006). This has an impact on DNA methylation genome-wide (Ren et al., 2019; Yu et al., 2014a). Besides altering epigenetic features and the expression of transposable elements (TE), HELLS absence in mouse tissues (brain and liver) and in fibroblasts has very limited consequences on gene expression (Huang et al., 2004; Yu et al., 2014b). In Hells KO mouse oocytes, the DNA methylation level of some TE families is reduced and their expression is increased; however, the expression of several meiotic genes is not affected (De La Fuente et al., 2006). The consequences of Hells deficiency on DNA methylation and expression have not been tested in spermatocytes. However, in the absence of HELLS, major epigenomic alterations in non-repeated DNA are not expected during meiosis, and consistently, H3K4me3 level at promoters is not altered in Hells cKO spermatocytes (Spruce et al., 2020).

The implication of 5-hydroxymethylcytosine at meiotic DSB sites

The presence of 5hmC at DSB hotspots was first reported by Brick and colleagues (Brick et al., 2018) using genome-wide data on cytosine methylation and hydroxyl-methylation patterns in mouse spermatocytes, mainly at the pachytene stage (Hammoud et al., 2014). Here, we found that this DNA modification is also present at hotspots earlier in meiosis, at leptotene-zygotene stages, when DSB formation takes place. By assessing 5hmC in mouse strains that carry different Prdm9 alleles (Prdm9^Dom2 and Prdm9^Cst), we found that 5hmC deposition depends on PRDM9 DNA-binding specificity. Moreover, we detected 5hmC enrichment in a narrow window of about +/- 250bp around the center of PRDM9-binding sites. Remarkably, PRDM9 binding is not sufficient and PRDM9 methyltransferase activity also is required for 5hmC enrichment. As we showed that 5hmC presence at hotspots does not require SPO11, we propose that 5hmC is promoted by a PRDM9-dependent chromatin modification step before DSB formation (Figure 5C). Therefore, 5hmC is a new feature of the local signature of active hotspots, like the histone modifications H3K4me3, H3K4me36 and H3K9ac (Buard et al., 2009; Davies et al., 2016; Grey et al., 2017; Lam et al., 2019; Powers et al., 2016).

The next question concerns the mechanism of the 5hmC enrichment at PRDM9-dependent hotspots. This enrichment is not observed in somatic tissues (Brick et al., 2018), which is consistent with the PRDM9 dependency we observed and with the PRDM9-specific expression at the leptotene stage of the meiotic prophase (Jung et al., 2019; Spruce et al., 2020). In the mouse male germline, a high level of DNA methylation is induced genome-wide during germline development in spermatogonia before meiosis entry and is maintained during meiotic prophase with a transient reduction at preleptonema (Gaysinskaya et al., 2018). A similar high DNA methylation level is observed at meiotic DSB sites (Figure 5—figure supplement 1D; Chen et al., 2020). Therefore, it could be hypothesized that a TET enzyme promoting the conversion of 5mC to 5hmC (Ito et al., 2010) is recruited upon or concomitantly with PRDM9 binding to its sites. One possible scenario could be that TET recruitment involves HELLS. Indeed, HELLS can interact with one, two, or all three TET enzymes, depending on the cell type (MCF-7 cells, HEK293T, mouse embryonic stem cells) (de Dieuleveult et al., 2020; Jia et al., 2017), and co-localize with 5hmC when stably expressed in HK1 cells (Jia et al., 2017). As no evidence of HELLS/TET interaction in meiotic cells is available, a PRDM9-dependent chromatin modification might be implicated in recruiting the putative TET activity. ZCWPW1, a reader of H3K4me3 and H3K36me3 that is required for efficient DSB repair (Huang et al., 2020; Mahgoub et al., 2020; Wells et al., 2019), might be directly or indirectly involved in this recruitment.

The function of 5hmC at meiotic hotspots is unknown. At least two non-exclusive consequences of 5hmC can be envisioned. First, as 5hmC has been associated with sites of open chromatin, such as active and poised enhancers, in several cell types (Sérandour et al., 2012; Stroud et al., 2013; Szulwach et al., 2011), it could have an active role in recruiting partners or stabilizing interactions, similarly to the recruitment of factors described in neuronal progenitor cells (Spruijt et al., 2013). Second, it has been shown that 5hmC prevents the binding of several methyl-CpG-binding proteins (Jin et al., 2010). One or both of these consequences of the conversion of 5mC to 5hmC could have a positive effect on DSB repair at meiotic hotspots in male meiosis. We favor the second scenario, in which the conversion of 5mC to 5hmC allows antagonizing the binding of factors with affinity for 5mC and which could interfere with meiotic recombination. Indeed, it is difficult to reconcile a positive role for 5hmC with the observation that DSB formation and repair is efficient at hotspots without CpGs in spermatocytes, and at all hotspots in oocytes, which have a low global level of cytosine methylation (Seisenberger et al., 2012).

The control of initiation sites of meiotic recombination by PRDM9 underlies a sophisticated regulation that goes beyond the simple binding to specific DNA motifs in the genome. Clearly, our findings and those from Baker’s laboratory (Spruce et al., 2020) indicate that the control of chromatin is an important step for DSB formation and repair. PRDM9 and HELLS drive epigenetic modifications before and independently of DSB formation, setting the stage for downstream steps. Not only histone modifications but also DNA methylation appears to be a potential additional level of regulation of meiotic recombination, with potential distinct consequences during male and female meiosis where some differences in hotspot activity have been detected (Brick et al., 2018) and from the analysis of 5hmC in the male germ line presented in this study. These observations also highlight the need of understanding the sex-specific features of meiotic recombination in general.

Materials and methods

Key resources table

Reagent type (species) or resource	Designation	Source or reference	Identifiers	Additional information
Mouse strains
	C57BL/6JOlaHsd	Envigo	C57BL/6JOlaHsd	Named B6
	B10.MOLSGR(A)-(D17Mit58-D17Jcs11)/Bdm (RJ2)	Grey et al., 2009	MGI:5319075	Named RJ2
	B6;129P2 < Prdm9tm1Ymat>/J	Hayashi et al., 2005	MGI:3624989	Named Prdm9 KO
	Spo11 < tm1Mjn>	Baudat et al., 2000	MGI:2178805	Named Spo11 KO
	Hells < tm1a(EUCOMM)Wtsi/Ieg>	EUCOM Bradley et al., 2012	MGI:4431905
	C57BL/6 Tg(CAG-Flpo)1Afst	Kranz et al., 2010	MGI:4453967
	C57BL/6 Tg(CMV-cre)1Cgn	Schwenk et al., 1995	MGI:2176180
	Tg(Stra8-icre)1Reb/J <(Stra8-iCre)>	Sadate-Ngatchou et al., 2008	MGI:3779079
	Tg(RP23-159N6*)23Bdm	Diagouraga et al., 2018	MGI:5565212	Named B6-Tg(YF)
Cell lines
	HeLa	ATCC	HeLa S3 ATCC CCL-2.2
Yeast strains
	AH109	James et al., 1996		S. cerevisiae
	Y187	Harper et al., 1993		S. cerevisiae
Recombinant DNA reagents
	PRDM9A-Flag-HA-Nt into retroviral pOZ-FH-N vector	This study	N/A	Vector from Addgene DB3781
	PRDM9A-Flag-HA-Ct into retroviral pOZ-FH-C vector	This study	N/A	Vector from Addgene cat# 32516
	pGAD GH for fusion to Gal4 activation domain, modified for Gateway cloning	Van Aelst et al., 1993	Clontech No. 638853	LEU2 marker
	pAS2dd for fusion to Gal4 DNA-binding domain, modified for Gateway cloning	Fromont-Racine et al., 1997		TRP1 marker
	pB29 for PRDM9 (aa 1–511) expression fused to LexA for yeast two-hybrid screen	Hybrigenics
Antibodies
	Guinea-pig anti-SYCP3	Grey et al., 2009	N/A	Home-made WB: 1/2000 IF: 1/500
	Rabbit anti-SYCP1	Abcam	Cat# ab15090 RRID:AB_301636	IF: 1/400
	Rabbit anti-DMC1	Santa Cruz	Cat# scH100 RRID:AB_2277191	IF: 1/200
	Goat anti-DMC1	Santa Cruz	Cat# scC20 RRID:AB_2091206	ChIP: 24 µg
	Rabbit anti-HELLS	Novus	Cat# NB 100–278 RRID:AB_350198	WB: 1/2000 IF: 1/200
	Mouse monoclonal anti-HELLS	Santa Cruz	Cat# sc46665 RRID:AB_627895	IF: 1/100
	Mouse monoclonal anti-phospho-histone H2AFX (Ser139)	Millipore	Cat# MP05-636 RRID:AB_309864	Named γH2AFX IF: 1/10000
	Rabbit anti-Gal4 activation domain (GAD) (Millipore, 06–283)		Now at Sigma-Aldrich Cat# ABE476	WB: 1/3000
	Rabbit anti-Gal4 DNA-Binding domain	Sigma–Aldrich	Cat# G3042 RRID:AB_439688	WB: 1/2000
	Rat monoclonal anti-Tubulin [YOL1/34]	Abcam	Cat# ab 6161 RRID:AB_305329	WB: 1/3000
	Rabbit anti-5hmC	Active Motif	Cat# AM 39791 RRID:AB_2630381	hMeDIP: 5 µg
	Rabbit anti-PRDM9	Grey et al., 2017	N/A	Home-made WB: 1/2000 IF: 1/200 ChIP: 4 µg
	Rabbit anti-H3K4me3	Abcam	ab8580 RRID:AB_306649	ChIP: 4 µg
	Goat anti-rabbit IgG-HRP	Pierce	Cat# 1858415 RRID:AB_1185567	WB: 1/10000
	Goat anti-Guinea-pig IgG-HRP	Jackson Immuno Research	Cat# 706-035-148 RRID:AB_2340447	WB: 1/3000
	Goat anti-rabbit IgG-Alexa 555	Thermo Fisher Scientific	Cat# ab150078 RRID:AB_2535849	IF: 1/400
	Goat anti-guinea-pig IgG-Alexa 488	Thermo Fisher Scientific	Cat# ab150185 RRID:AB_2534117	IF: 1/400
	Donkey anti-mouse IgG-Alexa 680	Thermo Fisher Scientific	Cat# ab175774 RRID:AB_2534014	IF: 1/100
	Donkey anti-mouse IgG-Alexa 647	Thermo Fisher Scientific	Cat# ab150107 RRID:AB_162542	IF: 1/400
Oligonucleotides
	Genotyping Hells cKO mice, see Supplementary file 2	This study
	RT-qPCR, see Supplementary file 3	This study, Buard et al., 2009, Diagouraga et al., 2018	N/A
Commercial assays or kits
	DeadEnd Fluorometric TUNEL System	Promega	Cat# G3250
	Anti-HA beads	Santa Cruz	Cat# sc-500773
	EZview anti-FLAG M2 Affinity Gel	Sigma–Aldrich	Cat# F2426
	hMeDIP Kit	Actif Motif	Cat# AM55010
	NEB Next Ultra Library Preparation Kit	New England Biolabs	Cat# NEB7370S
	ChIP-IT High Sensitivity Kit	Actif Motif	Cat# AM53040
	MMLV-based retroviral transduction system	Nakatani and Ogryzko, 2003	N/A
Chemical compounds
	HA peptide	Covance	Cat #PEP-101P-1000
	FLAG peptide	Sigma	Cat #F4799
	Optiprep Idoixanol	Sigma–Aldrich	Cat# D1556
	Sytox Green	Thermo Fisher Scientific	Cat# S70020
	WIN 18466	Tocris Bioscience	Cat# 4736	Hogarth et al., 2013
	Retinoic Acid	Sigma–Aldrich	Cat# R2625
Deposited data
	Mass spectrometry proteomics	ProteomeXchange Consortium	Dataset identifier PXD017337
	NGS SSDS ChIP (DMC1) and hMeDIP	GEO	GSE145768
Softwares and Algorithms
	Bowtie 2		http://bowtie-bio.sourceforge.net/bowtie2/index.shtml
	Modified BWA algorithm	Khil et al., 2012	N/A
	Tim Galore!		https://www.bioinformatics.babraham.ac.uk/projects/trim_galore/
	Bismark		https://www.bioinformatics.babraham.ac.uk/projects/bismark/
	Bedtools suite		https://bedtools.readthedocs.io/en/latest/content/bedtools-suite.html

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HELLS is co-immunoprecipitated with PRDM9.

Table 1—source data 1

HELLS interacts with PRDM9.

Meiotic prophase is defective in Hells cKO spermatocytes.

Figure 2—source data 1

HELLS is required for the formation of meiotic DSBs at sites of PRDM9-dependent DSB formation; DSBs are directed at default sites in the absence of HELLS.

Figure 3—source data 1

5hmC is enriched at PRDM9-dependent sites and correlates with PRDM9 occupancy.

5hmC enrichment at DSB sites sorted by CpG content and model.

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Yukiko Imai

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Mathilde Biot

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Julie AJ Clément

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Mariko Teragaki

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Serge Urbach

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Thomas Robert

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Frédéric Baudat

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Corinne Grey

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Bernard de Massy

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