Paternal contributions to epigenetic inheritance are not well understood. Paternal contributions via marked nucleosomes are particularly understudied, in part because sperm in some organisms replace the majority of nucleosome packaging with protamine packaging. Here we report that in Caenorhabditis elegans sperm, the genome is packaged in nucleosomes and carries a histone-based epigenetic memory of genes expressed during spermatogenesis, which unexpectedly include genes well known for their expression during oogenesis. In sperm, genes with spermatogenesis-restricted expression are uniquely marked with both active and repressive marks, which may reflect a sperm-specific chromatin signature. We further demonstrate that epigenetic information provided by sperm is important and in fact sufficient to guide proper germ cell development in offspring. This study establishes one mode of paternal epigenetic inheritance and offers a potential mechanism for how the life experiences of fathers may impact the development and health of their descendants.
Epidemiological studies in humans and experiments in mammalian models have revealed that conditions experienced by fathers can affect future generations1,2. However, the mechanisms by which fathers transmit information beyond the DNA code, in other words epigenetic information, to future generations are not well understood. Paternal contributions via chromatin marking are especially mysterious. This is partly because sperm DNA in some organisms is repackaged with protamines and with reduced levels of histones, complicating analysis of the sperm epigenome and challenging the notion that marked histones in sperm may provide epigenetic memory. Advances in genomics have enabled researchers to decipher the epigenetic landscape of sperm from humans, mice, and zebrafish3,4,5,6,7. Those studies demonstrated that the sperm genome retains histones, although the extent varies from 1–10% in mammals to 100% in zebrafish. Retained histones are modified with active and/or repressive histone modifications, unveiling the potential for sperm to transmit epigenetic information to offspring.
The presence of modified histones in sperm raises important questions. Can sperm transmit epigenetic information to offspring in the form of histone modifications? What is the fate of sperm-inherited marking in early embryos? Does sperm-inherited marking impact offspring development? C. elegans offers an exceptional system in which to address these questions. C. elegans lacks DNA methylation on cytosines8, one established mediator of epigenetic control, and thus may rely more heavily on histone modifications to transmit epigenetic information. Indeed, C. elegans sperm retain at least some histone packaging of the genome9,10,11, deliver chromosomes marked with histone modifications to embryos9,10,11, and can transmit a chromatin-based memory of temperature, diet, and stress to offspring12,13,14. Here we analyzed the epigenome of C. elegans sperm and tested whether epigenetic information in the form of marked nucleosomes influences germline development in offspring.
Here we document that C. elegans sperm retain modified histones genomewide, similar to zebrafish sperm, and that sperm carry a histone-based epigenetic memory of genes with spermatogenesis-restricted expression and unexpectedly also genes with oogenesis-enriched expression. In sperm, spermatogenesis-restricted genes are marked with an unusual combination of active and repressive histone modifications, which may be a sperm-specific signature and which resolves to retention of only repressive marks in early embryos. We find that genes previously shown to have enriched expression during oogenesis are also transcribed during spermatogenesis and thus bear active marks as a result of their transcription. We demonstrate that sperm marking is important for normal germ cell development in offspring whose germ cells inherit both sperm and oocyte chromosomes, and sufficient for normal germ cell development in offspring whose germ cells inherit only sperm chromosomes. Our studies establish modified histones retained in mature sperm as one mechanism by which fathers may transmit heritable traits, and highlight a role for sperm epigenetics in the development and fertility of descendants.
C. elegans sperm retain nucleosomes genome-wide
To determine how the genome is packaged in C. elegans sperm, we isolated adult males and collected mature sperm (~ 99% purity, Supplementary Fig. 1a). We utilized micrococcal nuclease digestion followed by paired-end sequencing (MNase-seq) to evaluate the presence of nucleosomes across the genome in sperm. We found that sperm retain nucleosomes across all six chromosomes, comparable in presence and gross distribution to early embryos but with half the MNase-seq reads from the X chromosome in sperm compared to early embryos, as expected based on their different X:A ratios (Supplementary Fig. 2a-b). Genome-wide retention of nucleosomes in C. elegans sperm resembles zebrafish sperm and differs from mammalian sperm, which replace 90–99% of their histone packaging with protamine packaging3,4,5,6,7.
To analyze the distribution of histone modifications across the genome in C. elegans sperm, we solubilized formaldehyde-fixed mononucleosomes from sperm and performed chromatin immunoprecipitation followed by sequencing (ChIP-seq). We focused on a modification associated with gene repression (trimethylation of histone H3 on Lys27, H3K27me3) and two modifications associated with gene expression (H3K36me3 and H3K4me3), because these modifications have been implicated in transgenerational epigenetic inheritance in C. elegans9,11,14,15,16,17,18. We found that C. elegans sperm retain modified histones across all six chromosomes with alternating H3K36me3- and H3K27me3-marked chromatin domains across the five autosomes (Fig. 1, Supplementary Fig. 2c). This domain organization is similar to that observed in early embryos15,19: H3K36me3 domains span the coding regions of single genes or sets of adjacent genes, and H3K27me3 domains overlie silent genes and intergenic regions. The level of H3K4me3 was lower in sperm compared with early embryos. We conclude that in C. elegans sperm the genome is packaged with nucleosomes bearing histone modifications.
To gain a comprehensive view of the epigenome transmitted to embryos by both gametes, we profiled oocyte chromatin using ChIP-seq analysis. As wild-type oocytes cannot be obtained in sufficient quantities for ChIP-seq, we profiled chromatin from ovulated but unfertilized oocytes collected from feminized worms. These oocytes were estimated to be 90–95% pure with slight contamination from gonads and immature oocytes (Supplementary Fig. 1b, Methods). Ovulated but unfertilized oocytes from feminized worms were previously shown to display changes in RNA accumulation compared to wild-type oocytes20. We observed similar changes with our oocyte preparations from feminized worms and determined those changes to be mainly downregulation of germline genes and upregulation of somatic genes, typical of an embryogenesis program. Nevertheless, the chromatin in those oocytes still displays histone marking consistent with oocytes: 84% of genes expressed during oogenesis (called “oogenesis genes”, ref. 21 and Methods) bear the active mark H3K36me3, and 86% bear the active mark H3K4me3 (Supplementary Fig. 3d, e); 81% of soma-specific genes (Methods) and 83% of strict embryo genes22 bear the repressive mark H3K27me3 (Supplementary Fig. 3d, e). We conclude that ChIP-seq data from our oocyte preparations largely reflect oocyte chromatin states.
Sperm display multivalent marking on spermatogenesis genes
Comparison of ChIP-seq data revealed that sperm, oocytes, and early embryos display very similar chromatin domains marked with either H3K36me3 or H3K27me3 (Fig. 1b, Fig. 2a–c, the second ChIP-seq replicate is shown in Supplementary Fig. 4). To ask whether genes are marked with H3K36me3, H3K27me3, both, or neither, we calculated the mean normalized ChIP signal for each protein-coding gene over the gene body and displayed the values in scatter plots. In all three cell types, sperm, oocytes, and early embryos, the majority of genes appear in the top-left and the bottom-right quadrants, as expected, showing that 86% of all genes are marked with either H3K27me3 or H3K36me3 (Supplementary Fig. 5, gray). To correlate marking of genes with their transcription status in adult germlines, we profiled by RNA sequencing (RNA-seq) the transcriptome of spermatogenic and oogenic germlines. We found that genes expressed in both spermatogenic and oogenic germlines (called “sex-independent genes”, Methods) are generally marked with the active modification H3K36me3 and lack the repressive modification H3K27me3 (Fig. 2a–c). Genes that are not transcribed in either spermatogenic or oogenic germlines (called “silent genes”, ref. 23 and Methods) are marked with the repressive modification H3K27me3 only (Fig. 2a, b). In short, genes expressed in both spermatogenic and oogenic germlines are marked with H3K36me3, and genes silent in both are marked with H3K27me3, following an “either H3K36me3 or H3K27me3” rule, consistent with the known antagonism between H3K36me3 and H3K27me324,25.
A surprising exception to the “either H3K36me3 or H3K27me3” rule is spermatogenesis genes in sperm. These are genes expressed exclusively in spermatogenic germlines and not in oogenic germlines (“spermatogenesis-specific genes” or “spermatogenesis genes” for short, Supplementary Fig. 3a, Methods). Strikingly, these genes (as well as previously defined sperm-enriched genes21,26) display both H3K36me3 and H3K27me3 over their gene body in sperm (Fig. 2a–c). Also surprising is the presence of another active histone modification, H3K4me3, over the body of spermatogenesis genes in sperm (Fig. 2a, b, d); that mark typically appears as a sharp peak at the promoter of expressed genes. Taken together, our data suggest that in sperm spermatogenesis genes are marked with both active (H3K36me3 and H3K4me3) and repressive (H3K27me3) marks, which we refer to as “multivalent” marking. In oocytes, spermatogenesis genes bear only H3K27me3 as expected, as they are not expressed during oogenesis (Fig. 2b–d). In early embryos, spermatogenesis genes also bear only H3K27me3 (Fig. 2), suggesting that the two active modifications transmitted from sperm are lost or erased in early embryos. We conclude that sperm carry a history of spermatogenesis gene expression using an unusual combination of histone modifications.
Sperm display active histone marks on oogenesis genes
Another class of genes with unexpected marking in sperm is genes with oogenesis-enriched expression (“oogenesis-enriched genes” or “oogenesis genes” for short21,26; Methods). Some gene products from this class are directly involved in oogenesis (e.g., the yolk receptor RME-2), whereas others are maternally synthesized and oocyte-supplied gene products involved in early embryo development (e.g., EGG-4, PIE-1, PAR-6, and NOS-2). We expected these genes to be transcriptionally repressed in male germlines and to bear H3K27me3 in sperm. Unexpectedly, we found that in sperm 78% of oogenesis genes are instead marked with H3K36me3 and 75% with H3K4me3, and are devoid of H3K27me3, typical of expressed genes (Fig. 3a–c, Supplementary Fig. 3c–e). We consider two possible mechanisms by which such oogenesis genes exhibit active epigenetic states in sperm. Marking of oogenesis genes is: (1) maternally inherited and maintained in males or (2) generated de novo in male germlines in a transcription-dependent manner. To test the latter, we analyzed our germline RNA-seq data and found that 73% of oogenesis genes (82% of those bearing the active mark H3K36me3 in sperm) are indeed transcribed in spermatogenic germlines (i.e., have Reads Per Kilobase of transcript per Million mapped reads (RPKM) values > 15 in Fig. 3d, Methods). As an independent method to test this and to visualize spatiotemporal patterns of expression, we employed single-molecule fluorescence in situ hybridization (smFISH)27, using probes against well-known oogenesis messenger RNAs (pie-1, par-6, nos-2, mex-3, and cpg-2). smFISH indeed detected transcripts from these genes in spermatogenic germlines, especially during pachytene (Fig. 3e, Supplementary Fig. 6). As expected, oogenesis genes display active histone modifications in oocyte ChIP-seq and show smFISH signal in oogenic germlines (Fig. 3, Supplementary Fig. 3d,e, Supplementary Fig. 6). Our observation that many oogenesis genes are transcribed in male germlines is consistent with other published findings: (1) during spermatogenesis in hermaphrodites, the RNA-binding proteins FOG-1 and FOG-3, which promote sperm cell fate, predominantly associate with oogenic transcripts28, and (2) males contain many small RNAs that guide the activity of the Argonaute protein CSR-1 and that are antisense to oogenic transcripts29. Indeed, we were not able to identify a high-confidence set of “oogenesis-specific genes” (i.e., expressed in oogenic germlines and not in spermatogenic germlines) using the same criteria we used to identify “spermatogenesis-specific genes” (Supplementary Fig. 3c, Methods). Thus, most oogenesis genes are transcribed in male germlines, perhaps to maintain those genes in an open chromatin state in sperm. We conclude that sperm carry a histone-based epigenetic memory of spermatogenesis gene expression, which includes (1) spermatogenesis genes bearing multivalent marking and (2) genes well known for their expression during oogenesis bearing active marking.
Sperm chromatin is important for the fertility of offspring
Our observation that sperm chromosomes are marked in a manner that reflects germline gene expression prompted the question whether sperm chromatin marking is important for germline development in offspring. To address this, we analyzed the fertility of worms that inherited sperm chromosomes lacking a histone modification thought to be important for epigenetic memory. The three histone modifications that have been implicated in epigenetic memory in C. elegans are methylated H3K4, H3K36, and H3K279,11,14,15,16,17,18. The first two marks each rely on multiple histone methyltransferases15,16 and are challenging to completely deplete from sperm. Consequently, we focused on H3K27me3, which can be eliminated from sperm chromosomes by disrupting Polycomb Repressive Complex 2 (PRC2) in males11,30. Males homozygous for a null mutation in mes-3, which encodes a subunit of the worm PRC2 complex, were mated with feminized mes-3/ + heterozygous worms to produce offspring that inherited sperm chromosomes lacking H3K27me3 (Fig. 4a). High percentages of the resulting mes-3 homozygous (92%) and heterozygous (73%) offspring developed into sterile adults in this sensitized genetic background (Fig. 4b, red, M + P- for Maternally marked chromosomes and Paternal chromosomes lacking marking, Methods). In contrast, genetically identical control offspring that received H3K27me3-marked sperm chromosomes displayed low sterility (Fig. 4b, blue, M + P + ). This suggests that paternally transmitted epigenetic information is important for germline development in offspring.
We next analyzed gene expression changes in the germlines of M + P − offspring that show high sterility and investigated whether they reflect sperm transmission of altered chromatin states or an altered cargo of mRNAs. The germlines of M + P − offspring displayed mainly upregulation of somatic genes and genes on the X chromosome, as previously documented in M + Z − (Maternal load of MES protein, no Zygotic synthesis) mes mutant germlines24. We compared the transcriptomes of mes-3 male germlines (parent germlines), mes-3 sperm, and germlines from M + P − offspring, along with their respective controls (Fig. 4c, d). We found significant overlaps between genes with altered mRNA accumulation in parent germlines and in sperm (p < 10−70, hypergeometric test in R), and between genes upregulated in parent germlines and in germlines in M + P − offspring (p < 10−5) (Fig. 4c). We did not observe a significant overlap between genes with altered mRNA accumulation in sperm and in germlines in M + P − offspring (p = 0.4) (Fig. 4c). These findings suggest that at least some genes upregulated in parent germlines are also upregulated in the germlines of M + P − offspring, and that an altered cargo of mRNAs in mutant sperm does not mediate this. This is further supported by density plot analyses of three sets of genes identified in these RNA-seq experiments: 123 genes upregulated in mes-3 parent germlines and in mes-3 sperm, 439 genes upregulated in mes-3 parent germlines but not in mes-3 sperm, and 81 genes upregulated in mes-3 sperm but not in mes-3 parent germlines (Fig. 4d). The two gene sets upregulated in parent germlines (plus or minus sperm) were statistically significantly upregulated in the germlines of M + P − offspring when compared with all genes, whereas the gene set upregulated only in sperm was not significantly upregulated in the germlines of M + P − offspring. These findings suggest that mes-3 mutant sperm convey a memory of gene upregulation to the next generation not via an altered payload of mRNAs but perhaps via altered chromatin states.
Sperm chromatin is sufficient for the fertility of offspring
Given that sperm chromosomes are marked in a manner that reflects both spermatogenic and oogenic gene expression patterns, that epigenetic marking of sperm chromosomes is faithfully transmitted through embryo cell divisions11, and that sperm epigenetic marking is important in offspring, we next tested whether sperm epigenetic marking alone is sufficient for proper development of the germline in offspring. We utilized a mutant that, during the first embryonic division, delivers the sperm genome to the daughter cell that generates the germline and the oocyte genome to the other daughter cell31. This mutant overexpresses GPR-1, a protein involved in regulation of kinetochore pulling forces. GPR-1 overexpression results in excessive pulling forces, causing the paternal and maternal pronuclei to inappropriately move to opposite poles of the one-cell embryo instead of merging in the center of the embryo. In this mutant background, ~ 60% of offspring undergo atypical chromosome segregation, generating mosaic embryos whose germlines are derived entirely from sperm chromosomes, and ~ 40% of offspring undergo normal chromosome segregation31. To track the parental genomes, differentially tagged histone transgenes were used31: a green fluorescent protein (GFP)-tagged histone H2B encoded in the sperm genome and a TdTomato-tagged histone H2B encoded in the oocyte genome (Fig. 5a). Remarkably, we found that mosaic embryos whose germline inherited only sperm chromosomes (“red-head” worms) develop into fertile adults (as observed in ref. 31) with a normal brood size, similar to control worms (“yellow” worms) in which the germline inherited both sperm and oocyte chromosomes (Fig. 5b). RNA-seq analysis demonstrated that the germline transcriptome of “red-head” worms and their offspring show few ( < 80 genes) and minor changes compared with control worms (Fig. 5c). These findings demonstrate that epigenetic information provided by sperm can guide proper germ cell development. Our findings are consistent with those of ref. 32 that showed that offspring that inherit both homologs of a marked autosome from the oocyte or the sperm are viable and fertile, indicating that C. elegans autosomes lack imprinting. Indeed, it appears likely that either oocyte-derived or sperm-derived chromosomes can support normal development31,32.
C. elegans sperm resemble zebrafish sperm in retaining nucleosomes genome-wide. In contrast, mammalian sperm replace 90–99% of their nucleosome packaging with protamine packaging. We note that protamine-like proteins have been identified in C. elegans10,33. It is possible that in C. elegans sperm some regions are packaged with a mixture of histones and protamines, as suggested by analysis of mammalian sperm3,7,34.
Multivalent marking of spermatogenesis-specific genes in C. elegans sperm reflects colocalization by ChIP of the assayed histone modifications, the active marks H3K4me3 and H3K36me3 and the repressive mark H3K27me3. There are at least three possible explanations for this colocalization by ChIP: (1) active and repressive marks coexist on the same H3 tails, (2) active and repressive marks exist on different H3 tails of the same nucleosomes, and (3) active and repressive marks exist on different nucleosomes in the population analyzed. Further studies are required to distinguish between these possibilities.
Intriguingly, multivalent marking of genes with methylated H3K4, H3K36, and H3K27 was also observed in zebrafish sperm6. This may be a sperm-specific chromatin signature. Mammalian sperm bear domains of methylated H3K4 and H3K27, similar to bivalent domains observed in embryonic stem cells3,4,5,7,35. In both zebrafish and mammalian sperm, multivalency is associated with genes that are silent during spermatogenesis but expressed during embryo development, suggesting that unique chromatin states in sperm poise certain genes for later expression in embryos. In contrast, multivalency in C. elegans sperm is associated with genes that are transcribed during spermatogenesis but are silent in mature sperm and in embryos. We speculate that multivalent marking in C. elegans sperm serves a different function than in zebrafish and mammalian sperm, namely to enable an epigenetic memory of spermatogenesis to be reset. Our previous studies suggest that an epigenetic memory of germline gene expression transmitted from sperm and oocytes is maintained by the histone H3K36 methyltransferase MES-4, which is recruited to and maintains high levels of methylated H3K36 on germline-expressed genes in embryos, to help instruct primordial germ cells how to develop15. The finding that abnormal retention of an epigenetic memory of spermatogenesis compromises germline health36 suggests that sperm epigenetic marking must be reset each generation. We speculate that this is achieved in early embryos by removal or loss of active marks (H3K4me3 and H3K36me3) from spermatogenesis-specific genes, to avoid propagating a memory of their expression, and by retaining repressive marks (H3K27me3) on those genes, to keep them repressed until spermatogenesis commences at a later stage. Multivalent marking of chromatin domains may serve diverse functions depending on biological context, developmental tissue and stage, and organism.
Our study demonstrates that C. elegans sperm transmit epigenetic information in the form of marked histones, and that this sperm-transmitted information influences development of the next generation. Although mammalian sperm retain a low level of histone packaging, several findings suggest that even mammalian sperm transmit histone-based epigenetic information. First, as noted above, modified histones are retained on developmentally important loci in human and mouse sperm, perhaps to influence expression of those loci in offspring3,4,7. Second, single-generation exposure of rats to toxicants resulted in altered patterns of histone retention in sperm in future generations, raising the possibility of transmission of environmental effects in mammals via histone packaging in sperm37. Comparisons across organisms continue to shed light on diverse mechanisms of transgenerational epigenetic inheritance and how the life experiences of fathers may impact the development and health of their descendants.
C. elegans strains and culture conditions
All strains were cultured on NGM (Nematode Growth Medium) agar plates at 20 °C, unless otherwise noted, using standard methods. CF512 and SS1167 were maintained at 15 °C, and HBR1280 and HBR1281 were maintained at 24 °C. The following strains were used: N2 (Bristol) as wild type, CB1489 him-8(e1489) IV, CF512 rrf-3(b26) II; fem-1(hc17ts) IV, DH245 fem-2(b245ts) III, SS818 mes-3(bn35) I/hT2-GFP (I;III), SS1167 mes-3(bn35) I/hT2-GFP (I;III); fem-2(b245ts) III, HBR1280 oxTi75[eft-3p::GFP::H2B::tbb-2 3′UTR + unc-18( + )], HBR1281 oxTi411[eft-3p::TdTomato::H2B::unc-54 3′UTR + Cbr-unc-119( + )] III; ddIs32[yfp::gpr-1(synthetic, CAI 1.0, artificial introns)].
Isolation of C. elegans males and purification of sperm
The following protocols were partially adapted from refs. 33,38. These protocols isolate highly enriched populations of spermatids, which have compacted nuclei that have completed meiotic division but have not developed motility structures to form motile spermatozoa. As these cells have undergone sperm-specific DNA compaction, we refer to these spermatids as mature sperm or “sperm” for short throughout the text. Mature sperm from C. elegans were collected and purified from him-8(e1489) males. A mutation in him-8 causes X chromosome non-disjunction during meiosis and thus generates a high percentage (~ 30%) of males39. Large cultures of him-8(e1489) worms (5–10 million) were synchronously grown from starved L1s in fernbach flasks containing S medium and HB101 Escherichia coli, shaking at 270 r.p.m. at 20 °C for ~ 62 h (MaxQ 3000 Benchtop shaker, Barnstead Lab-Line). The mixture of gravid hermaphrodites and adult males (day 1 adults) was collected using a separatory funnel. An equal volume of worm suspension and 60% ice-cold sucrose was mixed in a 25 mL tube and centrifuged for 5 min at 1000 × g. Worms contained in the top-layer were collected on 20-micron Nytex mesh (CellMicroSieves, BioDesign, Inc.) and rinsed with S-basal, after which males were allowed to wiggle through the mesh for at least for 30 min; gravid hermaphrodites remained on top of the mesh. The males were transferred to a 15-micron mesh, rinsed with S-basal several times to remove any larvae and small debris, and collected from the top of the mesh. Filtering of males was repeated twice to yield 10–15 mL packed males of > 98% purity as determined under a dissecting microscope. Males were resuspended in 20 mL freshly prepared Squash Medium (50 mM HEPES, 1 mM MgSO4, 70 mM choline chloride, 5 mM CaCl2, 1 mM phenylmethylsulfonyl fluoride, 1 mg/mL bovine serum albumin, 190 mOsm, pH 6.5), centrifuged for 5 min at 1000 × g and settled on ice, and excess Squash Medium was removed. The packed males were pressed 2 mL at a time using a custom-made “Sperminator” apparatus: males were evenly placed on one Plexiglass “squash plate”, a second “squash plate” was placed on top, and the two plates were pressed gently together using the “Sperminator” at 1000 psi for 10 s to squeeze sperm out of male worms, while preserving intact worms to prevent contamination from ruptured worm tissues. The collected sperm were filtered through 20-, 15-, 10-, and two rounds of 5-micron Nytex mesh to eliminate contamination by non-sperm cells and spermatocytes. Purified sperm were collected in a 1.5 mL eppendorf tube by centrifugation (1700 × g for 5 min), rinsed with Squash Medium, and again filtered through a 5-micron mesh. Sperm quantity (20–100 million sperm) was quantified using a hemocytometer, and sperm purity (~ 99%) was estimated by microscopic analysis (DIC imaging and DNA staining). Pelleted sperm were flash frozen in liquid nitrogen and kept at −80 °C.
Preparation of sperm chromatin for ChIP
Frozen sperm (10~50 million) were thawed on ice, rinsed once in 1 mL chilled Micrococcal Nuclease (MNase) Buffer (50 mM HEPES pH 7.5, 110 mM NaCl, 40 mM KCl, 2 mM MgCl2, 1 mM CaCl2), and fixed in 1 mL freshly prepared Fix Solution (1% formaldehyde in MNase Buffer) for 52 s, while constantly pipetting up and down. After adding glycine (final 125 mM) to stop cross-linking, sperm were rinsed once with 1 mL chilled MNase Buffer. Fixed sperm were treated with Lysis Buffer (final 0.2% NP-40 and 0.5% sodium deoxycholate) for 5 min on ice and digested with MNase for 5 min at 37 °C at a density of 0.1 million sperm per μL (5 units of MNase per 1 million sperm). To each tube, EDTA (final 10 mM), protease inhibitor (Roche, #04693159001, final 1 × after a tablet was resuspended in water), and Triton X-100 (final 1%) were added, and each tube was nutated at 4 °C for at least 2 h to facilitate chromatin solubilization. The digested sperm chromatin was mixed with two volumes of 150 mM salt FA Buffer (50 mM of HEPES pH 7.5, 1 mM EDTA pH 7.4, 1% Triton X-100, 0.1% sodium deoxylcholate, 150 mM NaCl) and treated with a Covaris S2 model (duty cycle 20%, intensity 8, cycle per burst 200, 60 s per cycle, total 5 cycles) to liberate sperm chromatin from the insoluble material. The entire content was transferred to a 1.5 mL siliconized tube, and centrifuged at 16,000 × g for 15 min at 4 °C. The supernatant, which contains fragmented and soluble sperm chromatin, was transferred to a new siliconized tube, flash frozen in liquid nitrogen, and stored at − 80 °C. Agarose gel electrophoresis (1.2% stained with SYBR Green) and an Agilent 2100 Bioanalyzer System were used to confirm that the majority of soluble chromatin was in mononucleosomes.
ChIP-seq from sperm
Soluble sperm chromatin from ~ 3.3 million sperm was thawed on ice, brought up to 110 μL with 150 mM salt FA Buffer supplemented with sarkosyl (final 1%). As “input” 10 μL was saved. To the remaining 100 μL soluble sperm chromatin, 1 μg antibody was added, and ChIP was performed using an IP-Star Compact Automated System (Diagenode) according to the manufacturers’ instructions with the following settings and reagents: “indirect method” with 100 μL reaction, 80 μL DynabeadsTM (M-280, sheep anti-mouse IgG, Life Technologies); IP for 12 h, bead incubation for 2 h; 10 min washes at middle speed with 1 M salt FA Buffer, 500 mM salt FA Buffer, TEL Buffer (0.25 M LiCl, 1% NP-40, 1% sodium deoxycholate, 1 mM EDTA, 10 mM Tris-HCl, pH 8), and TE Buffer (10 mM Tris-HCl pH 8.0, 1 mM EDTA); elution in Elution Buffer (1% SDS and 250 mM NaCl in 1X TE). Both IP and “input” were brought up to 300 μL with Elution Buffer with 1.5 μL 20 mg/mL proteinase K and incubated for 2 h at 55 °C and then overnight at 65 °C to reverse crosslinks. The next day, the magnetic beads were removed from the ChIP samples using a magnetic stand and sperm DNA was extracted using phenol–chloroform extraction, using the Phase Lock Gel system (5 PRIME #2302810). Sperm DNA was precipitated overnight at − 80 °C in ethanol with glycogen as carrier, and the resulting DNA pellets were resuspended in 15 μL nuclease-free water. One third of the DNA (5 μL) was used for ChIP-quantitative PCR (qPCR) to check ChIP efficiency, and libraries were prepared from the remaining 10 μL ChIP and “input” DNA using MicroPlex Library Preparation kit v2 (Diagenode, #C05010012). A real-time qPCR machine (Roche LightCycler 480) was used to monitor library amplification to avoid overamplification. Size selection was performed after library amplification using AMPure XP beads (Beckman Coulter, A63881) to enrich for 100–300 bp inserts. The final libraries were evaluated using an Agilent 2100 Bioanalyzer System (High Sensitivity DNA Analysis kit) and Quant-iT assay (Invitrogen, high-sensitivity double-stranded DNA). The multiplexed libraries were sequenced on either HiSeq4000 or HiSeq2500 rapid platforms at the Vincent J. Coates Genomics Sequencing Laboratory at University of California, Berkeley.
Isolation of C. elegans oocytes
The following protocols were partially adapted from refs. 40,41,42. C. elegans oocytes were collected and purified from hermaphrodites feminized by temperature-sensitive mutations in fem-1 and rrf-3 (previously known as fer-15) in strain CF51243. At the restrictive temperature, mutant hermaphrodites fail to make sperm and accumulate unfertilized oocytes in the uterus. Synchronized L1 larvae from CF512 were plated on 40–60 High Growth (HG) plates (2% peptone, 51 mM NaCl, 25 mM potassium phosphate, 5 μg/mL cholesterol, 1 mM CaCl2, 1 mM MgCl2, 2.5% agar) seeded with E. coli OP50 and grown for ~ 55 h at 15 °C until worms reached late L3 stage. Worms were then upshifted to 25 °C for 24–36 h to feminize them. Visual inspection under a dissecting microscope confirmed that day 1 feminized adults contained only unfertilized oocytes, and that no fertilized embryos or L1 larvae were present on the plates. Approximately 1 million feminized adults were washed from the HG plates with Egg Salts Buffer (25 mM HEPES pH 7.4, 118 mM NaCl, 48 mM KCl, 2 mM CaCl2, 2 mM MgCl2), and washed 3 × in a 50 mL conical tube to remove excess E. coli and other debris. After washing, worms were pelleted by centrifugation, excess buffer was removed, and densely packed worms were transferred to a 15 cm petri dish on ice. Worms were chopped with a clean razor blade for 5 min, until extruded gonads and liberated oocytes were visible under a dissecting microscope. Oocytes and carcass fragments were poured over a 45-micron mesh (NTX45, Dynamic Aqua-Supply LTD). Oocytes passed through the mesh, while carcass fragments remained above the mesh. The flow-through was filtered through a 20-micron mesh to collect oocytes above the mesh, while smaller debris went through the mesh. An aliquot of unfixed oocytes was saved for 4′,6-diamidino-2-phenylindole (DAPI) staining and RNA isolation to estimate the quality and purity, measured as the number of oocytes/total cells in multiple fields of view under a dissecting microscope. The purity of the first and second replicates was > 95% and > 90%, respectively. Oocytes were fixed in 2.2% formaldehyde in Egg Salts Buffer for 5 min, quenched in 125 mM glycine to stop cross-linking, and then washed twice in M9 Buffer (3 g KH2PO4, 6 g Na2HPO4, 5 g NaCl, H2O to 1 L). Fixed oocytes were pelleted, flash frozen in liquid nitrogen, and stored at − 80 °C.
ChIP-seq from oocytes
Fixed oocytes (0.5–1 million) were thawed on ice and resuspended in chilled MNase Buffer. Oocytes were sonicated for 5 cycles with a tip sonicator (5 rounds of 5 s on and 25 s off). Following sonication, oocytes were pre-warmed to 25 °C for 5 min, followed by addition of 250 units MNase. A pilot digestion time-course experiment was performed to identify the optimal digestion time, which yielded the majority of chromatin as mononucleosomes, as measured by Agilent bioanalyzer analysis. As a result of the pilot experiment, oocyte chromatin was digested with MNase for 50 min. Digestion was halted by addition of EDTA (final 10 mM) and incubated on ice for 5 min. Protease inhibitor (Roche, #04693159001, final 1 × in water), Triton X-100 (final 1%), and sodium deoxycholate (final 0.1%) were added to the digested oocyte chromatin. The oocyte chromatin extract was split into separate aliquots, and ChIPed in parallel with different antibodies. Dynabeads were washed 3 × with cold FA Buffer. Each antibody (1 μg) was nutated with beads at 4 °C for ~ 2 h. After saving 40 μL oocyte extract as “input,” oocyte extract was added to the beads, supplemented with sarkosyl (1% final), and nutated overnight at 4 °C. The next day, the beads were washed twice in FA Buffer, once in 1 M salt FA Buffer, 500 mM salt FA Buffer, and TEL Buffer, and then twice in TE Buffer. Immunocomplexes were eluted from the beads by incubation with Elution Buffer at 65 °C for 15 min with gentle vortexing. RNA was digested with RNase A for 1 h at room temperature, followed by proteinase K treatment for 2 h at 55 °C. Crosslinks were reversed by incubation at 65 °C overnight, followed by phenol–chloroform extraction, and DNA precipitation in ethanol with linear acrylamide at − 80 °C for 4 h. ChIPed oocyte DNA was resuspended in 15 μL nuclease-free water. Oocyte libraries were prepared with the NEBNext Ultra DNA library Prep Kit (NEB) following the manufacturers’ instructions. AMPure beads were used for size selection after amplification to enrich for fragments corresponding to mononucleosomes. Libraries were sequenced on an Illumina HiSeq2500 platform at the Princeton High Throughput Sequencing Facility.
ChIP-seq from early embryos
Data are from ref. 19.
Antibodies used for ChIP
Mouse monoclonal antibodies for H3K36me3 (HK00001, now marketed as Wako MABI0333, #300–95289), H3K27me3 (HK00013, now marketed as Wako MABI0323, #309–95259), and H3K4me3 (Wako MABI0304, #305–34819) are described in ref. 44 and were validated as in ref. 45.
Analysis of ChIP-seq data
Raw sequence reads from the Illumina HiSeq (50 bp single-end reads) were mapped to the C. elegans genome (Wormbase version WS220) using Bowtie with default settings46. MACS2 was used to call peaks and to create bedgraph files with the following settings: -g ce --bdg --keep-dup = auto --broad --broad-cutoff = 0.01 --nomodel --extsize = 25047. Bedgraph files were scaled to 10 million total autosomal reads (X chromosome reads were not included for scaling, due to the different X:A ratios between sperm, oocytes, and early embryos) and converted to bigwig using the bedGraphToBigWig UCSC Genome Browser tool48. These were displayed in the UCSC Genome Browser (visibility = full, autoScale = off, windowingFunction = Mean + whiskers, smoothingWindow = 2). To display gene-level ChIP signal in scatter plots (e.g., Fig. 2c), the mean read coverage for each protein-coding gene was calculated using the bigWigAverageOverBed UCSC Genome Browser tool48 using WS220 gene start and end annotations. For H3K4me3, a histone mark typically found in promoters, the read coverage was calculated from 500 bp upstream of the gene start annotation to 500 bp downstream. These gene read coverages were log2 transformed after a pseudo-count of 1 was added. To account for slightly varying background noise levels in the different ChIP-seq samples, the gene read coverages were z-scored based on the average and standard deviation of all autosomal gene read coverages. Specifically, the read coverages for all genes were centered by subtracting the average of the read coverages of autosomal genes and then divided by the standard deviation of the autosomal gene read coverages. One adaptation was made for H3K27me3: the 30th percentile of autosomal gene read coverage, instead of the average, was chosen as the baseline signal and was subtracted from all gene read coverages genome-wide. This is because H3K27me3 occupies ~ 2/3 of the C. elegans genome and the autosomal average gene read coverage did not seem like an appropriate baseline to center the H3K27me3 ChIP signal. The Principal Component Analysis in Supplementary Fig. 4d was performed on these z-scored autosomal gene read coverages. The prcomp function in R was used. Metagene analysis was performed using the R package “SeqPlots” with default settings49.
Sperm were fixed as described for sperm ChIP-seq, and 1–2 million sperm were digested with increasing amounts of MNase for 5 min at 37 °C. Early embryos were harvested from hermaphrodites that contained only a couple of embryos and fixed as described in ref. 15 . Early embryos (500–750 μL) were thawed on ice and resuspended in 2 mL of Dounce Buffer (0.35 M sucrose, 15 mM HEPES pH 7.5, 0.5 mM EGTA, 0.5 mM MgCl2, 10 mM KCl, 0.1 mM EDTA, 1 mM dithiothreitol, 0.5% Triton X-100) supplemented with protease inhibitors (Roche, #04693159001) and dounce-homogenized ~ 10 times until the majority of embryos were disrupted. The homogenized embryos were spun at 380 × g for 1 min at 4 °C and the supernatant containing nuclei was transferred to a new tube. This was repeated one more time. The nuclei contained in the supernatant were collected by centrifugation at 4000 × g for 10 min at 4 °C and resuspended in MNase Buffer. Approximately 5 million embryo nuclei were digested with increasing amounts of MNase at 37 °C for 30 min. Digested chromatin from sperm and early embryos was reverse-crosslinked overnight at 65 °C in Elution Buffer supplemented with 1.5 μL 20 mg/mL proteinase K. DNA was extracted using phenol–chloroform. The degree of MNase digestion was assessed using agarose gel electrophoresis and an Agilent 2100 Bioanalyzer. Illumina sequencing libraries were constructed with DNA extracted from the mononucleosome-enriched digestions that were comparable between sperm and early embryos, using NEBNext Ultra DNA Library Prep Kit (NEB, E7370). During library construction, size selection was performed on adaptor-ligated DNA before amplification to remove fragments larger than 250 bp (40 μL of AMPure beads were used for First Bead Addition based on the manufacturers’ instructions), and PCR-amplified DNA was purified using 1:1 AMPure XP beads, which removed fragments smaller than 100 bp. The final libraries were evaluated using an Agilent 2100 Bioanalyzer System and Quant-iT assay, and were sequenced at the Vincent J. Coates Genomics Sequencing Laboratory at University of California, Berkeley (50 bp paired-end read sequencing).
Analysis of MNase-seq data
Paired-end MNase-seq reads were mapped to the C. elegans genome (Wormbase version WS220) using Bowtie with default settings46. After mapping, fragments smaller than 140 bp were filtered out using bamtools 2.5.150. Bedtools51 was used to scale the remaining mapped fragments to 10 million autosomal reads and to generate bedgraph files. As for ChIP-seq, the bedGraphToBigWig tool was used to convert the bedgraph files to bigwig format. Bigwig files were displayed in the UCSC genome browser (visibility = full, autoScale = off, windowingFunction = Mean, smoothingWindow = 2). To assess whether there are nucleosome-occupancy differences in certain genomic regions between sperm and early embryos, the bigWigAverageOverBed UCSC Genome Browser tool48 was used to calculate the average MNase fragment coverage of 150 bp windows tiled every 50 bp and covering the whole genome for all sperm and embryo samples. Windows (150 bp) that had less than 1 fragment covering them in all four sperm and early embryo samples were excluded from further analysis, as these 150 bp windows cover genomic regions of very low mappability with the sequencing data available. About 2.2% of the genome was excluded this way. Density plots were made in R to show the distribution of 150 bp window fragment coverage for the autosomes and for the X chromosome for all four samples of sperm and early embryo MNase-seq. The analysis was repeated for 500 bp windows tiled every 250 bp, 1 kb windows tiled every 500 bp, 2 kb windows tiled every 1 kb, and 5 kb windows tiled every 2.5 kb.
For male spermatogenic germlines, samples were from N2 males (Figs. 2,3), CB1489 him-8(e1489) males (Figs. 2,3,4), and SS818 mes-3 (bn35) homozygous M + Z − males from heterozygous parents (M for maternal product and Z for zygotic product) (Fig. 4). For sperm, samples were from CB1489 him-8(e1489) males and SS818 mes-3(bn35) M + Z − males (Fig. 4). For hermaphrodite oogenic germlines, samples were from N2 (Figs. 2,3), DH245 fem-2(b245) (Figs. 2,3), SS1167 mes-3(bn35) (M + P − Z − and M + P + Z − where P is for paternal H3K27me3 by MES-3); fem-2(b245) (Fig. 4), HBR1280 oxTi75[eft-3p::GFP::H2B::tbb-2 3′UTR + unc-18( + )] (Fig. 5, control), “red-head” F1 progeny (from HBR1281 crossed with HBR1280; genetically identical to HBR1280) (Fig. 5), and F2 offspring from “red-head” F1s (genetically identical to HBR1280) (Fig. 5). Both spermatogenic and oogenic germlines were dissected from day 1 adults as described in ref. 24; 20–100 distal gonad arms were cut at the late-pachytene gonad bend. Mature sperm were released from adult males by cutting the males with a 30-gauge needle and collected with a pulled glass Pasteur pipette coated with Sigmacote (SL2 Sigma). Total RNA was extracted in TRIzol reagent (Invitrogen), ribosomal RNA was depleted using an NEBNext rRNA Depletion kit (E6310), and libraries were prepared using an NEBNext Ultra RNA Library Prep Kit for Illumina (E7530). Libraries were sequenced at the Vincent J. Coates Genomics Sequencing Laboratory at University of California, Berkeley (50 bp single-end read sequencing). For each genotype, 2–4 biological replicates were obtained. Sequence reads were processed as described in ref. 52. Briefly, TopHat253 was used to align the RNA-seq reads to the C. elegans transcriptome (WS220) with default parameters. HTSeq54 was used to obtain read counts per transcript (HTseq counts). Differentially expressed genes were determined with DESeq255 in R using HTSeq counts and a FDR < 0.05 as the significance cutoff. RPKMs were calculated by dividing HTseq counts by exonic transcript length obtained from Wormbase and scaling the total read counts per sample to 1 million reads. If a gene had multiple transcript isoforms, the longest was chosen. For Fig. 3d and Supplementary Fig. 3a,c, RPKMs were log transformed after adding a pseudo-count of 1. Genes with RPKM > 15 were called ‘expressed’ based on the expression of defined spermatogenic and oogenic gene sets (see below) in spermatogenic and oogenic germlines.
Single-molecule fluorescence in situ hybridization
smFISH analysis was performed on day 1 adult male and hermaphrodite gonads dissected from him-8(e1489) worms as in ref. 56. Biosearch Technologies designed, synthesized, and labeled the Stellaris probes. The pie-1, par-6, and nos-2 probes were coupled to Quasar 670, the mex-3 probe was coupled to Cal Fluor Red 590, and the cpg-2 probe was coupled to Cal Fluor Red 610. Each probe was resuspended in 250 μL of TE Buffer pH 8.0 and then further diluted to 1:30 for hybridization. The microscope and its settings are as in ref. 52. Fig. 3 and Supplementary Fig. 6 contain montages generated by splicing together contiguous images acquired with identical settings. Male and hermaphrodite pairs used identical confocal settings, with the exposure optimized for visualizing the male gonads. All images were processed identically with ImageJ and Adobe Illustrator. For both oogenic and male germlines, 10–60 gonads were visually examined under the microscope and at least 3 germlines were imaged in 1–3 separate experiment(s).
Measurement of fertility/sterility
For Fig. 4, feminized heterozygous mes-3(bn35)/hT2-GFP; fem-2ts worms were obtained by shifting their mothers from 15 °C to 24 °C at the L4 larval stage and selecting GFP + offspring. Feminized worms were mated with either homozygous mes-3(bn35) M + Z −; fem-2ts males or heterozygous mes-3(bn35)/hT2-GFP; fem-2ts males raised at 15 °C, and the fertility/sterility of their offspring grown at 15 °C was visually scored under the microscope. We found that having fem-2ts and mes-3 heterozygous in the mother’s genotype is essential for paternal-effect sterility, and thus represents a sensitized genetic background. Unpaired unequal-variance one-tailed Student’s t-tests were performed to calculate the significance of % sterile worms between the genetically identical M + P − vs. M + P + offspring.
Measurement of brood size
For Fig. 5, strain maintenance and experiments with HBR1280 and HBR1281 were performed at 24 °C, because the transgenes in these strains are prone to gene silencing. Cross-progeny from the matings shown in the figure were scored using a fluorescence microscope to identify those that arose from normal vs. atypical segregation. The numbers of their offspring that grew to adults were scored. We censored 1–3 worms per experiment that died prematurely during the reproductive period (days 1–4 of adulthood) due to the vulva bursting, internal hatching of F1 offspring (bag of worms), or contamination of plates.
All gene sets are in Supplementary Data 1.
- Spermatogenesis genes (i.e., spermatogenesis-specific genes): RPKM in spermatogenic germlines (from either wild-type or him-8 males) > 15, RPKM in wild-type oogenic germlines < 1, and DESeq2 FDR < 0.05 for significance of higher expression in spermatogenic compared to oogenic germlines. Spermatogenic germlines from wild-type males compared to oogenic germlines identified 1369 genes, and him-8 males compared with oogenic germlines identified 1330 genes. The 1298 spermatogenesis-specific genes that overlapped between the two comparisons were used in our analyses. The 1298 spermatogenesis genes we defined included 690 of the 827 genes defined in Reinke et al.21. The 2498 spermatogenesis genes defined by Ortiz et al.26 included 1206 of our 1298 genes.
- Sex-independent genes: RPKM in spermatogenic germlines (from either wild-type or him-8 males) > 5, RPKM in oogenic germlines > 5, FDR > 0.05, and log2 (fold change) < 2 (genes with no significant differential expression between spermatogenic and oogenic germlines). Spermatogenic germlines from wild-type males compared with oogenic germlines identified 2549 genes, and spermatogenic germlines from him-8 males compared with oogenic germlines identified 2472 genes. The 2097 overlapping genes from these two comparisons were used in our analyses.
- Soma-specific genes (1171 genes) are genes expressed in at least 1 of 3 somatic tissues (muscle, gut, or neuron) with at least 8 SAGE tags57 but not enriched21 or detectably expressed58 in the adult germline.
- Silent genes are 410 serpentine receptor genes that are expressed in a few mature neurons and are not expected to be expressed in germlines, originally defined in23.
Statistical analysis and sample sizes for all experiments are described in figure legends. Student’s t-test was performed using Excel. Mann–Whitney U-test and hypergeometric test were performed using R. At least 2 biological replicates of sequencing data (ChIP/MNase/RNA-seq) were obtained; sample sizes were based on experience and the standards in the field. We omitted sequencing data generated and analyzed during the optimization phase of the project. The final samples included were those generated after optimization. DESeq2 was used to test for differential expression by use of negative binomial generalized linear models. Adjusted p-values were calculated by DESeq2 using the Benjamini–Hochberg method.
Raw sequence reads and processed data generated or reanalyzed in this study (MNase-seq, ChIP-seq, and RNA-seq) are in the NCBI GEO database, accession number GSE115709. All gene sets (see above) are in Supplementary Data 1. Other data used in this study are available at the NCBI GEO database, accession numbers GSE715-GSE737 (ref. 21), GSE57109 (ref. 26), ArrayExpress: E-TABM-598 (ref. 23), http://elegans.bcgsc.ca/home/sage.html (ref. 57), and http://tock.bcgsc.ca/cgi-bin/sage160 (ref. 58).
Klosin, A. & Lehner, B. Mechanisms, timescales and principles of trans-generational epigenetic inheritance in animals. Curr. Opin. Genet. Dev. 36, 41–49 (2016).
Rando, O. J. Intergenerational transfer of epigenetic information in sperm. Cold Spring Harb. Perspect. Med. 6, a022988 (2016).
Hammoud, S. S. et al. Distinctive chromatin in human sperm packages genes for embryo development. Nature 460, 473–478 (2009).
Brykczynska, U. et al. Repressive and active histone methylation mark distinct promoters in human and mouse spermatozoa. Nat. Struct. Mol. Biol. 17, 679–687 (2010).
Erkek, S. et al. Molecular determinants of nucleosome retention at CpG-rich sequences in mouse spermatozoa. Nat. Struct. Mol. Biol. 20, 868–875 (2013).
Wu, S. F., Zhang, H. & Cairns, B. R. Genes for embryo development are packaged in blocks of multivalent chromatin in zebrafish sperm. Genome Res. 21, 578–589 (2011).
Jung, Y. H. et al. Chromatin states in mouse sperm correlate with embryonic and adult regulatory landscapes. Cell Rep. 18, 1366–1382 (2017).
Simpson, V. J., Johnson, T. E. & Hammen, R. F. Caenorhabditis elegans DNA does not contain 5-methylcytosine at any time during development or aging. Nucleic Acids Res. 14, 6711–6719 (1986).
Arico, J. K., Katz, D. J., van der Vlag, J. & Kelly, W. G. Epigenetic patterns maintained in early Caenorhabditis elegans embryos can be established by gene activity in the parental germ cells. PLoS. Genet. 7, e1001391 (2011).
Samson, M. et al. The specification and global reprogramming of histone epigenetic marks during gamete formation and early embryo development in C. elegans. PLoS Genet. 10, e1004588 (2014).
Gaydos, L. J., Wang, W. & Strome, S. H3K27me and PRC2 transmit a memory of repression across generations and during development. Science 345, 1515–1518 (2014).
Klosin, A., Casas, E., Hidalgo-Carcedo, C., Vavouri, T. & Lehner, B. Transgenerational transmission of environmental information in C. elegans. Science 356, 320–323 (2017).
Tauffenberger, A. & Parker, J. A. Heritable transmission of stress resistance by high dietary glucose in Caenorhabditis elegans. PLoS Genet. 10, e1004346 (2014).
Kishimoto, S., Uno, M., Okabe, E., Nono, M. & Nishida, E. Environmental stresses induce transgenerationally inheritable survival advantages via germline-to-soma communication in Caenorhabditis elegans. Nat. Commun. 8, 14031 (2017).
Rechtsteiner, A. et al. The histone H3K36 methyltransferase MES-4 acts epigenetically to transmit the memory of germline gene expression to progeny. PLoS Genet. 6, e1001091 (2010).
Li, T. & Kelly, W. G. A role for Set1 / MLL-related components in epigenetic regulation of the Caenorhabditis elegans germ line. PLoS Genet. 7, e1001349 (2011).
Greer, E. L. et al. Transgenerational epigenetic inheritance of longevity in Caenorhabditis elegans. Nature 479, 365–371 (2011).
Furuhashi, H. et al. Trans-generational epigenetic regulation of C. elegans primordial germ cells. Epigenetics Chromatin 3, 15 (2010).
Ho, J. W. K. et al. Comparative analysis of metazoan chromatin organization. Nature 512, 449–452 (2014).
Stoeckius, M. et al. Global characterization of the oocyte-to-embryo transition in Caenorhabditis elegans uncovers a novel mRNA clearance mechanism. EMBO J. 33, 1751–1766 (2014).
Reinke, V., Gil, I. S., Ward, S. & Kazmer, K. Genome-wide germline-enriched and sex-biased expression profiles in Caenorhabditis elegans. Development 131, 311–323 (2004).
Baugh, L. R., Hill, A. A., Slonim, D. K., Brown, E. L. & Hunter, C. P. Composition and dynamics of the Caenorhabditis elegans early embryonic transcriptome. Development 130, 889–900 (2003).
Kolasinska-Zwierz, P. et al. Differential chromatin marking of introns and expressed exons by H3K36me3. Nat. Genet. 41, 376–381 (2009).
Gaydos, L. J., Rechtsteiner, A., Egelhofer, T. A., Carroll, C. R. & Strome, S. Antagonism between MES-4 and polycomb repressive complex 2 promotes appropriate gene expression in C. elegans germ cells. Cell Rep. 2, 1169–1177 (2012).
Yuan, W. et al. H3K36 methylation antagonizes PRC2-mediated H3K27 methylation. J. Biol. Chem. 286, 7983–7989 (2011).
Ortiz, M. A., Noble, D., Sorokin, E. P. & Kimble, J. A new dataset of spermatogenic vs. oogenic transcriptomes in the nematode. Caenorhabditis elegans. G3 4, 1765–1772 (2014).
Raj, A., van den Bogaard, P., Rifkin, S. A., van Oudenaarden, A. & Tyagi, S. Imaging individual mRNA molecules using multiple singly labeled probes. Nat. Methods 5, 877–879 (2008).
Noble, D. C. et al. Genomic analyses of sperm fate regulator targets reveal a common set of oogenic mRNAS in Caenorhabditis elegans. Genetics 202, 221–234 (2016).
Conine, C. C. et al. Argonautes promote male fertility and provide a paternal memory of germline gene expression in C. elegans. Cell 155, 1532–1544 (2013).
Bender, L. B., Cao, R., Zhang, Y. & Strome, S. The MES-2/MES-3/MES-6 complex and regulation of histone H3 methylation in C. elegans. Curr. Biol. 14, 1639–1643 (2004).
Besseling, J. & Bringmann, H. Engineered non-Mendelian inheritance of entire parental genomes in C. elegans. Nat. Biotechnol. 34, 982–986 (2016).
Haack, H. & Hodgkin, J. Tests for parental imprinting in the nematode Caenorhabditis elegans. MGG Mol. Gen. Genet. 228, 482–485 (1991).
Chu, D. S. et al. Sperm chromatin proteomics identifies evolutionarily conserved fertility factors. Nature 443, 101–105 (2006).
Wykes, S. M. & Krawetz, S. A. The structural organization of sperm chromatin. J. Biol. Chem. 278, 29471–29477 (2003).
Bernstein, B. E. et al. A bivalent chromatin structure marks key developmental genes in embryonic stem cells. Cell 125, 315–326 (2006).
Katz, D. J., Edwards, T. M., Reinke, V. & Kelly, W. G. A C. elegans LSD1 demethylase contributes to germline immortality by reprogramming epigenetic memory. Cell 137, 308–320 (2009).
Maamar, M. Ben, Sadler-Riggleman, I., Beck, D. & Skinner, M. K. Epigenetic transgenerational inheritance of altered sperm histone retention sites. Sci. Rep. 8, 5308 (2018).
L’Hernault, S. W. & Roberts, T. M. Cell biology of nematode sperm. Methods Cell Biol. 48, 273–301 (1995).
Hodgkin, J., Horvitz, H. R. & Brenner, S. Nondisjunction mutants of the nematode Caenorhabditis elegans. Genetics 91, 67–94 (1979).
Miller, M. A. Sperm and oocyte isolation methods for biochemical and proteomic analysis. Methods Mol. Biol. 351, 193–201 (2006).
Aroian, R. V., Field, C., Pruliere, G., Kenyon, C. & Alberts, B. M. Isolation of actin-associated proteins from Caenorhabditis elegans oocytes and their localization in the early embryo. EMBO J. 16, 1541–1549 (1997).
Luo, S., Kleemann, G. A., Ashraf, J. M., Shaw, W. M. & Murphy, C. T. TGF-β and insulin signaling regulate reproductive aging via oocyte and germline quality maintenance. Cell 143, 299–312 (2010).
Garigan, D. et al. Genetic analysis of tissue aging in Caenorhabditis elegans: A role for heat-shock factor and bacterial proliferation. Genetics 161, 1101–1112 (2002).
Liu, T. et al. Broad chromosomal domains of histone modification patterns in C. elegans. Genome Res. 21, 227–236 (2011).
Egelhofer, T. A. et al. An assessment of histone-modification antibody quality. Nat. Struct. Mol. Biol. 18, 91–93 (2011).
Langmead, B., Trapnell, C., Pop, M. & Salzberg, S. L. Ultrafast and memory-efficient alignment of short DNA sequences to the human genome. Genome Biol. 10, R25 (2009).
Zhang, Y. et al. Model-based analysis of ChIP-Seq (MACS). Genome Biol. 9, R137 (2008).
Kent, W. J., Zweig, A. S., Barber, G., Hinrichs, A. S. & Karolchik, D. BigWig and BigBed: enabling browsing of large distributed datasets. Bioinformatics 26, 2204–2207 (2010).
Stempor, P. & Ahringer, J. SeqPlots - interactive software for exploratory data analyses, pattern discovery and visualization in genomics. Wellcome Open Res. 1, 14 (2016).
Barnett, D. W. et al. BamTools: a C + + API and toolkit for analyzing and managing BAM files. Bioinformatics 27, 1691–1692 (2011).
Quinlan, A. R. & Hall, I. M. BEDTools: a flexible suite of utilities for comparing genomic features. Bioinformatics 26, 841–842 (2010).
Knutson, A. K., Rechtsteiner, A. & Strome, S. Reevaluation of whether a soma-to-germ-line transformation extends lifespan in Caenorhabditis elegans. Proc. Natl Acad. Sci. USA 113, 3591–3596 (2016).
Kim, D. et al. TopHat2: accurate alignment of transcriptomes in the presence of insertions, deletions and gene fusions. Genome Biol. 14, R36 (2013).
Anders, S., Pyl, P. T. & Huber, W. Genome analysis HTSeq — a Python framework to work with high-throughput sequencing data. Bioinformatics 31, 166–169 (2018).
Love, M. I., Huber, W. & Anders, S. Moderated estimation of fold change and dispersion for RNA-seq data with DESeq2. Genome Biol. 15, 550 (2014).
Lee, C. H., Sorensen, E. B., Lynch, T. R. & Kimble, J. C. elegans GLP-1/Notch activates transcription in a probability gradient across the germline stem cell pool. eLife 5, e18370 (2016).
Meissner, B. et al. An integrated strategy to study muscle development and myofilament structure in Caenorhabditis elegans. PLoS Genet. 5, e1000537 (2009).
Wang, X. et al. Identification of genes expressed in the hermaphrodite germ line of C. elegans using SAGE. BMC Genomics 10, 213 (2009).
We thank Strome lab members and A. Fire for helpful discussions, K. Kaneshiro for oogenic germline transcriptome data, E. Nishimura for some smFISH probes, H. Kimura for antibodies, D. Chu and J. Lieb for advice, and H. Bringmann for sharing gpr-1(oe) strains prior to publication. Some strains were provided by the CGC funded by NIH-P40OD010440. This work was supported by NIH-F32GM110892 to T.M.T., NIH-T32HG003284 to T.E.J., NIH-DP1GM119167 to C.T.M., and NIH-R01GM34059 to S.S., and used the QB3 Vincent J. Coates Genomics Sequencing Laboratory at UC Berkeley funded by S10OD018174.
The authors declare no competing interests.
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Tabuchi, T.M., Rechtsteiner, A., Jeffers, T.E. et al. Caenorhabditis elegans sperm carry a histone-based epigenetic memory of both spermatogenesis and oogenesis. Nat Commun 9, 4310 (2018). https://doi.org/10.1038/s41467-018-06236-8
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