1. Genetics and Genomics

PIE-1 SUMOylation promotes germline fates and piRNA-dependent silencing in C. elegans

  1. Heesun Kim
  2. Yue-He Ding
  3. Shan Lu
  4. Mei-Qing Zuo
  5. Wendy Tan
  6. Darryl Conte Jr
  7. Meng-Qiu Dong
  8. Craig C Mello  Is a corresponding author
  1. RNA Therapeutics Institute, University of Massachusetts Medical School, United States
  2. National Institute of Biological Sciences, China
  3. Howard Hughes Medical Institute, United States
https://doi.org/10.7554/eLife.63300
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Cite this article
  1. Heesun Kim
  2. Yue-He Ding
  3. Shan Lu
  4. Mei-Qing Zuo
  5. Wendy Tan
  6. Darryl Conte Jr
  7. Meng-Qiu Dong
  8. Craig C Mello
(2021)
PIE-1 SUMOylation promotes germline fates and piRNA-dependent silencing in C. elegans
eLife 10:e63300.
https://doi.org/10.7554/eLife.63300
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Abstract

Germlines shape and balance heredity, integrating and regulating information from both parental and foreign sources. Insights into how germlines handle information have come from the study of factors that specify or maintain the germline fate. In early Caenorhabditis elegans embryos, the CCCH zinc finger protein PIE-1 localizes to the germline where it prevents somatic differentiation programs. Here, we show that PIE-1 also functions in the meiotic ovary where it becomes SUMOylated and engages the small ubiquitin-like modifier (SUMO)-conjugating machinery. Using whole-SUMO-proteome mass spectrometry, we identify HDAC SUMOylation as a target of PIE-1. Our analyses of genetic interactions between pie-1 and SUMO pathway mutants suggest that PIE-1 engages the SUMO machinery both to preserve the germline fate in the embryo and to promote Argonaute-mediated surveillance in the adult germline.

Introduction

During every life cycle, the eukaryotic germline orchestrates a remarkable set of informational tasks that shape heredity and create variation necessary for the evolution of new species. One approach for understanding the mechanisms that promote germline specification and function has been the identification of genes whose protein products localize exclusively to the germline and for which loss-of-function mutations result in absent or non-functional germ cells and gametes (Seydoux and Braun, 2006). In Caenorhabditis elegans, PIE-1 is a key regulator of germline specification (Mello et al., 1992). The C. elegans zygote, P0, undergoes a series of asymmetric divisions that generate four somatic founder cells and the germline blastomere P4. The PIE-1 protein is maternally deposited and uniformly present in the cytoplasm and nucleus of the zygote, but rapidly disappears in each somatic blastomere shortly after division (Mello et al., 1996; Reese et al., 2000; Tenenhaus et al., 1998). In pie-1 mutants, the germline lineage differentiates into extra intestinal cells causing an embryonic arrest (Mello et al., 1992). PIE-1 localizes prominently in nuclei in the early P-lineage blastomeres and persists in the primordial embryonic germ cells through much of embryogenesis (Mello et al., 1996). The presence of PIE-1 correlates with global hypo-phosphorylation of the C-terminal domain (CTD) of RNA polymerase II (pol II) in germline blastomeres (Seydoux and Dunn, 1997), and some studies suggest that PIE-1 may directly inhibit the CTD kinase to prevent transcriptional activation (Batchelder et al., 1999; Ghosh and Seydoux, 2008).

PIE-1 is a member of the tandem CCCH zinc finger protein family (Blackshear et al., 2005). PIE-1 differs from most of its homologs in having a prominent nuclear localization. However, like the majority of its family members, PIE-1 also localizes in the cytoplasm where it is thought to bind and regulate the expression of germline mRNAs, including the nos-2 mRNA (Tenenhaus et al., 2001). Hints at the nuclear function of PIE-1 came from a yeast two-hybrid screen which identified the Krüppel-type zinc finger protein MEP-1 as a PIE-1 interacting factor (Unhavaithaya et al., 2002). MEP-1 co-purifies with LET-418, a homolog of mammalian ATP-dependent nucleosome remodeling factor Mi-2 (von Zelewsky et al., 2000), and with HDA-1, a homolog of mammalian histone deacetylase HDAC1 (Shi and Mello, 1998). Inactivation of maternal mep-1 and let-418 causes a striking developmental arrest of L1-stage larvae, whose somatic cells adopt germline-specific transcriptional programs, and assemble germline-specific peri-nuclear nuage-like structures called P granules (Unhavaithaya et al., 2002). These soma-to-germline transformations depend on the trithorax-related protein MES-4 and components of a polycomb repressive complex (PRC2) (MES-2 and MES-3) (Unhavaithaya et al., 2002), whose functions are thought to promote fertility by maintaining germline chromatin (Strome and Updike, 2015). Taken together, these previous studies on PIE-1 suggest that it functions as a master-regulator of the germline fate in C. elegans embryos, preventing somatic differentiation, while also protecting the germline chromatin from remodeling. However, the possible biochemical mechanisms through which this small CCCH zinc finger protein exerts its dual effects on transcription and chromatin in the germline were entirely unknown.

Here, we show PIE-1 promotes the regulation of its targets at least in part through the small ubiquitin-like modifier (SUMO). By yeast two-hybrid screening, we show that PIE-1 engages the highly conserved E2 SUMO ligase UBC-9. UBC-9 enzymes catalyze the addition SUMO to lysine residues on target proteins (Capili and Lima, 2007b; Geiss-Friedlander and Melchior, 2007; Johnson, 2004). The reversible addition of SUMO (or SUMOylation) and its removal by de-SUMOylating enzymes is thought to occur on thousands of substrate proteins with diverse functions, especially nuclear functions including DNA replication, chromatin silencing, and the DNA damage response (Hendriks and Vertegaal, 2016). SUMOylation can have multiple effects and is not primarily associated with the turnover of its targets, but rather is often associated with changes in protein interactions. For example, SUMOylation of a protein can promote interactions with proteins that contain SUMO-interacting motifs (Matunis et al., 2006; Psakhye and Jentsch, 2012; Shen et al., 2006).

Through a series of genetic and biochemical studies, we show that the SUMO pathway promotes the activity of PIE-1 in preserving the embryonic germline. We show that PIE-1 is itself modified by SUMO. Paradoxically, PIE-1 is not SUMOylated in early embryos, but rather in adult animals where PIE-1 was not previously known to be expressed or functional. Indeed, CRISPR-mediated GFP tagging of the endogenous pie-1 locus confirmed uniform nuclear expression of PIE-1 protein throughout the meiotic zone and in oocytes of adult hermaphrodites. Using whole proteome analysis for detecting SUMO-conjugated proteins, we identify the type 1 HDAC, HDA-1, as a protein modified by SUMO in a PIE-1-dependent manner. Surprisingly, whereas PIE-1 was originally thought to inhibit the MEP-1/Mi-2/HDA-1 complex in embryos, we show that in the germline PIE-1 acts in concert with the SUMO pathway to promote the association of MEP-1 with HDA-1, and to maintain the hypoacetylation of germline chromatin. Although pie-1 lysine 68 mutants that prevent PIE-1 SUMOylation are viable, we show that they exhibit synthetic lethality in combination with null alleles of gei-17, a Drosophila Su(var)2–10 SUMO-E3 ligase homolog (Hari et al., 2001; Mohr and Boswell, 1999; Ninova et al., 2020), and that double mutants exhibit potent desilencing of a piRNA Argonaute sensor. Our findings are consistent with a model in which PIE-1 engages SUMO to preserve the embryonic germline fate, and also to promote the assembly of a MEP-1/Mi-2/HDA-1 chromatin remodeling complex required for inherited Argonaute-mediated gene silencing in the adult hermaphrodite germline.

Results

PIE-1 is SUMOylated in adult germ cells

To explore how PIE-1 promotes germline specification, we sought to identify protein interactors. Immunoprecipitation of PIE-1 protein from embryo extracts proved to be challenging because the protein is expressed transiently in early embryos, where it is only present in early germline cells. Moreover, PIE-1 was insoluble and unstable in worm lysates preventing the analysis of PIE-1 complexes by immunoprecipitation (Figure 1—figure supplement 1). We therefore performed a yeast two-hybrid screen to identify PIE-1 interactors (Figure 1A and Supplementary file 1; see Materials and methods). As expected, this screen identified the Krüppel-type zinc finger protein MEP-1, a known PIE-1 interactor and co-factor of the Mi-2/NuRD (nucleosome remodeling deacetylase) complex (Passannante et al., 2010; Unhavaithaya et al., 2002). In addition, this screen identified the small ubiquitin-like modifier SMO-1 (SUMO); the E2 SUMO-conjugating enzyme UBC-9 (Jones et al., 2002); and GEI-17 (Holway et al., 2005; Kim and Michael, 2008), a homolog of vertebrate PIAS2 and Drosophila Su(var)2–10, an E3 SUMO ligase (Ninova et al., 2020; Pichler et al., 2017).

Figure 1 with 3 supplements see all
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PIE-1 is SUMOylated on K68 residue in the Caenorhabditis elegans germline.

(A) Summary of PIE-1 interactors identified by yeast two-hybrid screen (see Supplementary file 1 for complete list). (B and C) Domain structure of PIE-1 containing two zinc fingers (ZF1 and ZF2) and proline-rich region, and location (red bar) of a consensus small ubiquitin-like modifier (SUMO) acceptor motif (ψKXE, where ψ represents a hydrophobic amino acid, K is the acceptor lysine, and X is any amino acid) conserved in PIE-1 from other Caenorhabditis species. (D) Western blot analysis of SUMO-conjugated proteins in total worm lysates prepared with guanidine-HCl denaturing buffer or IP buffer. The resistant band (asterisk) migrates with the expected size of the E1 enzyme AOS-1, which attaches to SUMO by a thioester bond and may therefore resist SUMO proteases, which cleave isopeptide bonds. The black triangle indicates free SMO-1. (E and F) Western blot analyses of SUMOylated proteins enriched from (E) early embryo or (F) adult lysates from wild-type pie-1::flag or pie-1(K68R)::flag worms. SUMOylated proteins were enriched from worms expressing HIS10::SMO-1 by Ni-NTA chromatography. Black triangles indicate SUMOylated forms of PIE-1 or MRG-1. White triangles indicate unmodified PIE-1 or MRG-1. MRG-1 is a robustly SUMOylated protein (Supplementary files 2 and 3; Drabikowski et al., 2018; Kaminsky et al., 2009) and thus serves as a positive control. (G) Confocal images of PIE-1::GFP and mCherry::H2B in adult germline of live pie-1::gfp; pie-1p::mCherry::his-58 worms. Oocyte nuclei are indicated by white circles and numbered.

Motif analysis predicted one consensus SUMO acceptor site (ψKXE; Rodriguez et al., 2001) in PIE-1 that is perfectly conserved in PIE-1 orthologs of other Caenorhabditis species (Figure 1B and C). Although covalent in nature, the addition of SUMO to substrates is rapidly reversible by SUMO protease enzymes that are active under conditions typically used to prepare lysates for immunoprecipitation studies (Di Bacco et al., 2006; Zhang et al., 2017). For example, even the preparation and centrifugation of lysates at 4°C followed by reconstitution in IP buffer with no other incubation resulted in the complete removal of SUMO from its target proteins (Figure 1D). To identify SUMO-conjugated proteins, we inserted a poly-histidine epitope into the endogenous smo-1 gene, and then used nickel (Ni) affinity chromatography under stringent denaturing conditions to enrich SUMOylated proteins (Tatham et al., 2009). Eluates from Ni-affinity chromatography were then analyzed by mass spectrometry (MS) and western blotting (Figure 1—figure supplement 2B and C and see below).

In principle, it is possible to directly detect SUMOylated peptides by mass spectrometry (Impens et al., 2014; Knuesel et al., 2005). To create a cleavage signature suitable for high-throughput identification of modified peptide fragments, leucine 88 of SUMO must be substituted with lysine. Unfortunately, editing the endogenous smo-1 locus to encode the L88K mutation caused a lethal smo-1 phenotype in C. elegans (data not shown).

Previous proteomic analyses of SUMOylated worm proteins have relied on smo-1 transgenes that encode HIS-tagged SUMO fused to the FLAG epitope or to GFP (Drabikowski et al., 2018; Kaminsky et al., 2009). Inserting in-frame FLAG or mCherry sequences into the endogenous smo-1 locus caused pronounced hypomorphic smo-1 phenotypes (data not shown). We therefore inserted hexahistidine (HIS6) or decahistidine (HIS10) sequences directly after the initiator methionine codon of smo-1 without any other sequences. Both HIS fusions resulted in fully viable and healthy strains indistinguishable from wild type. We chose to use the HIS10 fusion because it was robustly conjugated to target proteins (Figure 1D) and allowed better retention to the Ni-NTA resin under stringent denaturing and washing conditions (Figure 1—figure supplement 2A, B and C).

The Ni-NTA resin retains non-SUMOylated protein species that are recovered even in the absence of HIS10::SUMO expression (e.g., see lanes 3 and 8 in Figure 1E and F). These non-SUMOylated proteins are not recovered via associations with SUMO-modified proteins but rather directly due to background binding of the individual denatured protein to the Ni-affinity matrix. The recovery of these background species from the matrix is not, therefore, a good measure of the actual ratio of SUMO-modified and -unmodified species in the lysate. The unavoidable recovery of unmodified species also impairs the sensitivity of MS as a means for identifying SUMO-modified proteins. Given the very high rate of false-negative detection in SUMO MS studies, we chose to apply the lowest possible arbitrary cut off of 1 spectral count enrichment over two controls—untagged SMO-1 and depletion of HIS10::SMO-1 by smo-1(RNAi)—when generating our list of candidate SUMO conjugates. This analysis identified 977 candidate SUMO (Supplementary file 2; see Supplementary file 3, Figure 1—figure supplement 2D, and Discussion section for comparison with previous studies). SUMOylated MRG-1, for example, was strongly enriched by Ni-affinity chromatography as detected by MS and western blot analyses (Supplementary file 2 and Figure 1E and F). Importantly, failure to detect a protein by SUMO proteomics should not be construed as evidence the protein is not modified or regulated by SUMO. For each candidate protein of interest, co-valent modification by SUMO should be assessed directly with the more sensitive approach of Ni-affinity chromatography and western blotting.

PIE-1 did not pass the arbitrary cut-off we applied to our MS data (Supplementary file 2). We therefore carefully monitored PIE-1 SUMOylation by western blotting. To do so, we inserted a sequence encoding the FLAG epitope into the endogenous pie-1 gene. The PIE-1::FLAG protein was expressed at similar levels in wild-type and his10::smo-1 worms (Figure 1E and F), and these worms were fully viable. Ni-affinity chromatography of embryo lysates failed to enrich a modified form of PIE-1::FLAG (Figure 1E). However, Ni-affinity chromatography of adult lysates enriched a slowly migrating form of PIE-1::FLAG protein that was ~12 kD larger than unmodified PIE-1::FLAG (compare lanes 14 and 19, Figure 1F). The modified PIE-1::FLAG band was absent when we mutated the presumptive SUMO acceptor site lysine 68 to arginine in PIE-1::FLAG (K68R) (Figure 1F, lane 20). Thus, lysine 68 is required for PIE-1 SUMOylation.

We were surprised to detect SUMOylated PIE-1 in adult hermaphrodites but not in embryos. Previous studies had only detected PIE-1 protein within embryonic germ cells and proximal oocytes of adult hermaphrodites (Reese et al., 2000; Tenenhaus et al., 1998). We therefore monitored PIE-1::GFP expressed from the endogenous pie-1 locus (Kim et al., 2014). As expected, in embryonic germ cells, PIE-1::GFP localized to nuclei, cytoplasm, and cytoplasmic P granules (i.e., P-lineage; Figure 1—figure supplement 3; Mello et al., 1996; Reese et al., 2000; Tenenhaus et al., 1998). In the adult pachytene germline, we found that PIE-1::GFP co-localized with chromosomes (as monitored by co-localization with mCherry histone H2B) and PIE-1 protein levels appeared to gradually increase during oocyte maturation (Figure 1G and Figure 1—figure supplement 3). These findings suggest that SUMOylation of PIE-1 occurs within a heretofore unexplored zone of PIE-1 expression within the maternal germline.

PIE-1 SUMOylation and SUMO pathway factors function together to promote fertility and embryonic development

To investigate the functional consequences of the K68R lesion, we performed a genetic complementation test with a previously described null allele, pie-1(zu154). In early embryos, maternal PIE-1 promotes the germ cell fate of the P2 blastomere and prevents P2 from adopting the endoderm and mesoderm fates of its somatic sister blastomere, EMS (Mello et al., 1992). Hermaphrodite worms homozygous for the loss-of-function pie-1(zu154) allele are fertile, but 100% of their embryos arrest development with extra pharyngeal and intestinal cells (Mello et al., 1992). By contrast, we found that most homozygous PIE-1(K68R) animals produce viable and fertile progeny but exhibit reduced fertility and increased embryonic lethality (Figure 2A and B), suggesting that the K68R lesion causes a partial loss of PIE-1 function. Consistent with this idea, further lowering pie-1 activity by placing the K68R allele over pie-1(zu154) dramatically enhanced the deficits in fertility (Figure 2A) and in embryo viability (Figure 2B). For example, about 11% of embryos produced by trans-heterozygotes failed to hatch (Figure 2B). When we examined a subset of the dead embryos by light microscopy, we found that 64% (14/22) arrested development with supernumerary intestinal cells, a hallmark of pie-1 loss of function (Mello et al., 1992). Thus, PIE-1(K68R) exhibits a partial loss of PIE-1 function.

Figure 2
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Genetic interactions between pie-1 and SUMO pathway.

(A) Brood size analysis and (B) embryonic lethality of wild-type (N2), pie-1(ne4303[K68R]), pie-1(zu154)/qC-1, and pie-1(ne4303[K68R])/pie-1(zu154). Statistical significance was determined by Wilcoxon-Mann-Whitney test: *p≤0.05; **p≤0.01; ****p≤0.0001. (C) Tests of genetic interactions between pie-1 and SUMO pathway mutants. Bar graphs show the percentage of dead embryos (gray) and percentage of dead embryos with extra intestine (yellow) among ‘n’ embryos scored. (D) Partial sequence alignment of UBC enzymes, including C. elegans UBC-9. Residues conserved in all UBC proteins are shown in red. Temperature-sensitive (ts) alleles of yeast Cdc34 result from mutations in highly conserved residues (blue boxes). Mutating the proline resides (P69S and P73S) resulted in non-conditional lethality in C. elegans. A G56R mutation in C. elegans UBC-9 caused a ts phenotype. (E) Location of the G56R mutation introduced into the endogenous ubc-9 gene by CRISPR genome editing. (F) Genetic interaction between pie-1 and ubc-9(ne4446[G56R]) allele at 25°C. Bar graphs show the percentage of embryos with extra intestine among ‘n’ embryos scored.

Figure 2—source data 1

Brood size and embryonic lethality.

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We reasoned that if the loss of SUMOylation is responsible for the hypomorphic phenotype of PIE-1(K68R) animals, then compromising the SUMO machinery might cause similar synthetic genetic interactions. To test this idea, we depleted the activity of each SUMO pathway gene by RNAi beginning at the L4 larval stage in wild-type and pie-1(zu154)/+ heterozygotes. RNAi at the L4 stage allows the worms to produce fertilized embryos depleted of SUMO activity. When exposed to control RNAi, both wild-type and pie-1(zu154) heterozygous worms produce 100% viable embryos (Figure 2C). RNAi targeting SUMO pathway factors (smo-1, gei-17, or ubc-9) caused wild-type and pie-1(zu154) heterozygous worms to make dead embryos. Whereas only 2–20% of embryos in the wild-type background made extra intestine, about 75% of embryos made by the pie-1(zu154) heterozygous worms arrested with extra intestinal cells (Figure 2C). The synergy between gei-17 and pie-1(zu154) was particularly striking: whereas gei-17(RNAi) in wild-type worms caused only 20% embryonic lethality, gei-17(RNAi) in pie-1/+ worms caused 82% of embryos to arrest development and 94% of these produced extra intestinal cells (Figure 2C).

In an effort to create temperature-sensitive (ts) alleles of endogenous ubc-9, we used genome editing to introduce point mutations corresponding to ts alleles of yeast ubc9 (Figure 2D and E; Betting and Seufert, 1996; Prendergast et al., 1995). One allele, ubc-9(ne4446), which encodes a G56R amino acid substitution, resulted in worms that were viable and fertile at the permissive temperature of 15°C, but inviable when shifted to the non-permissive temperature of 25°C. Some of the temperature-sensitive phenotypes of this allele can be reversed by shifting worms back to the permissive temperature (data not shown). When shifted to 25°C beginning at the L4 stage, ubc-9(ne4446[G56R]) worms developed into fertile adults that produced 100% dead embryos (n = 332) with defective body morphology but well-differentiated tissues. About 15% of ubc-9(ne4446[G56R]) embryos arrested with extra intestinal cells, consistent with previous studies showing that in smo-1(RNAi) and ubc-9(RNAi) embryos, the P2 blastomere expresses EMS-like cell lineage patterns, a pie-1 mutant phenotype (Santella et al., 2016). Strikingly, the proportion of arrested embryos with a pie-1-like phenotype was doubled when G56R homozygotes were shifted to 25°C in a heterozygous pie-1(zu154)/+ background (Figure 2F), supporting the idea that SUMO promotes the activity of PIE-1 in protecting the embryonic germline.

HDA-1 is SUMOylated in the adult

The finding that PIE-1 interacts with UBC-9, SMO-1, and GEI-17 in the yeast two-hybrid assay (Figure 1A and Supplementary file 1) raises the possibility that PIE-1 recruits the SUMO machinery to regulate its targets. If so, then one way to address the SUMO-dependent functions of PIE-1 is to search for proteins that are modified by SUMO in a PIE-1-dependent manner. To do this, we used RNAi to deplete PIE-1 from a synchronous population of young adult his10::smo-1 animals. As controls, we used RNAi targeting smo-1 and an empty RNAi vector (L4440). The depletion of PIE-1 and SMO-1 was monitored by western blot (Figure 3A). Ni-affinity chromatography followed by MS revealed 328 proteins that were reduced to a similar extent in lysates from both pie-1(RNAi) and smo-1(RNAi) animals (orange dots in Figure 3B and Supplementary file 4). Among this group of PIE-1-dependent SUMO targets, HDA-1 caught our attention because a previous study identified the nucleosome remodeling and deacetylase (NuRD) complex, including HDA-1/HDAC1 and its binding partners LET-418/Mi-2 and MEP-1, as potential targets of PIE-1 regulation (Unhavaithaya et al., 2002).

Figure 3
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PIE-1 SUMOylation promotes HDA-1 SUMOylation in the adult germline.

(A) Western blot showing relative levels of SUMOylation in HIS10::SMO-1 worms treated with control (L4440), pie-1(RNAi), or smo-1(RNAi). (B) Scatter plot comparing the levels of SUMOylated proteins in pie-1(RNAi) worms (x axis) and smo-1(RNAi) worms (y axis). Eluates from affinity chromatography of control, pie-1(RNAi), and smo-1(RNAi) lysates were analyzed by mass spectrometry. The log of the difference between spectral counts in control and mutant was plotted for each protein. Positive values represent proteins whose spectral counts were reduced in pie-(RNAi) and smo-1(RNAi). Negative values on the x axis represent proteins whose spectral counts increased in pie-1(RNAi) compared to control. Dashed lines indicate the position of a 1.5-fold difference between the changes in smo-1(RNAi) and pie-1(RNAi) worms. A full list of PIE-1-dependent SUMO targets is provided in Supplementary file 4. (C and D) Western blot analyses of SUMOylated HDA-1 (C) or MEP-1 (D) enriched from embryo (yellow background) or adult (blue background) lysates of wild-type, pie-1, or smo-1 mutants. Ni-NTA pull-downs are outlined by dashed red boxes. Black triangles indicate SUMOylated proteins; white triangles indicate unmodified proteins.

Figure 3—source data 1

Comparison the levels of SUMOylated proteins in pie-1(RNAi) with in smo-1(RNAi).

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To directly explore the possibility that PIE-1 promotes the SUMOylation of HDA-1 and MEP-1, we used Ni-affinity chromatography followed by western blotting. To monitor SUMOylation of MEP-1, we used CRISPR to insert tandem gfp and 3xflag coding sequences into the mep-1 gene—i.e., mep-1::gfp::tev::3xflag (mep-1::gtf). For HDA-1 detection, we used a previously validated antibody (Beurton et al., 2019). Western blot analyses of eluates from Ni-affinity chromatography experiments revealed that slowly migrating isoforms of HDA-1 (Figure 3C, lanes 11 and 16) were present in adult his10::smo-1 lysates, but absent from embryo lysates (Figure 3C, lane 5). By contrast, slowly migrating MEP-1 isoforms were present in both embryos and adults (Figure 3D, lanes 5, 11, and 16). These modified HDA-1 and MEP-1 isoforms were ~12 kD larger than unmodified HDA-1 and MEP-1, were only enriched by Ni-affinity chromatography of his10::smo-1 lysates, and were not detected in lysates prepared from smo-1(RNAi) worms (Figure 3C and D, lane 18), suggesting that the larger isoforms result from SUMOylation.

SUMOylated HDA-1 was not detected in extracts from pie-1(RNAi) adults (Figure 3C, lane 17) and appeared reduced in adult extracts from homozygous mutant animals expressing PIE-1(K68R) (Figure 3C, compare lanes 11 and 12). In contrast, MEP-1 SUMOylation was unaffected by genetic perturbations of pie-1 (Figure 3D, lanes 5, 12, and 17). Thus, SUMOylation of HDA-1 occurs only in adults and appears to depend—at least partly—on pie-1 activity and PIE-1 SUMOylation.

PIE-1 SUMOylation promotes formation of an adult germline MEP-1/HDA-1 complex

To address whether PIE-1 SUMOylation modulates the interaction of HDA-1 with other NuRD complex components, we immunoprecipitated MEP-1::GTF from early embryo and adult lysates using a GFP-binding protein (GBP) nanobody (Rothbauer et al., 2008) and detected LET-418 or HDA-1 by western blot. In embryo extracts, where PIE-1 and HDA-1 are not modified by SUMO, MEP-1 interacted with both LET-418 and HDA-1 (Figure 4, lanes 10 and 11). These robust interactions were not affected by the PIE-1(K68R) mutation (Figure 4, lane 12). In adult lysates, MEP-1 interacted robustly with LET-418, but only weakly with HDA-1 (Figure 4, lanes 22, 23, and 30). Despite a co-migrating background band present in control IPs from animals without MEP-1::GTF (see Figure 4, lanes 7, 8, and 9 longer exposures), this weak interaction between HDA-1 and MEP-1 was reproducibly detected, required both smo-1 and pie-1 activity (Figure 4, lanes 31 and 32), and was reduced in PIE-1(K68R) mutants (Figure 4, lane 24). Thus, SUMOylation of PIE-1 promotes a difficult to detect but reproducible interaction between HDA-1 and MEP-1 in the adult germline, but is not required for their much more robustly detected interaction in embryos. Given the transient nature of the SUMO modification, it is worth noting that if the interaction between HDA-1 and MEP-1 in adults requires the continued presence of HDA-1-SUMO, then our IP assays would likely underestimate the in vivo levels of the protein complex (see Discussion).

Figure 4
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PIE-1 SUMOylation is required for the assembly of MEP-1/HDA-1 complex in the adult germline.

Western blot analyses of proteins that immunoprecipitate with MEP-1::GTF from embryo (yellow background) or adult lysates (blue background) of wild-type, pie-1, or smo-1 mutant worms. MEP-1::GTF was immunoprecipitated with GFP nanobody (see 'Materials and methods'). Blots were probed with HDA-1, LET-418, or anti-FLAG (MEP-1::GTF) antibodies. Longer exposure of the HDA-1 blots shows the reduced interaction of HDA-1 with MEP-1 in pie-1 and smo-1 mutants.

PIE-1 suppresses histone acetylation and germline gene expression

If PIE-1 promotes the assembly of a functional HDA-1 NuRD complex in the adult germline, then we would expect global levels of acetylation to be increased in pie-1 mutant gonads. Indeed, immunostaining revealed increased levels of histone H3 lysine 9 acetylation (H3K9Ac) in pie-1 [K68R] gonads compared to wild-type gonads (Figure 5A and B), especially in the distal mitotic region and in oocytes. To more strongly deplete PIE-1 protein, we engineered an in-frame auxin-responsive pie-1::degron::gfp (see 'Materials and methods'). Exposing these animals to auxin from the L1 stage abolished PIE-1 expression in the adult germline (Figure 5—figure supplement 1) and caused a penetrant pie-1 maternal-effect embryonic lethal phenotype. Auxin-treated adult worms showed uniformly high levels of H3K9Ac throughout the germline (Figure 5A). Moreover, H3K9Ac levels were higher in oocytes of auxin-treated pie-1::degron::gfp worms than in oocytes of pie-1[K68R] worms (Figure 5B). These findings suggest that PIE-1(K68R) is compromised (but not completely inactive) for its ability to promote deacetylation of H3K9 in the adult germline.

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PIE-1 regulates histone H3K9Ac and spermatogenic genes in the adult germline.

(A) Immunofluorescence micrographs of H3K9Ac and DAPI staining in adult gonad of wild-type (wt), pie-1(ne4303[K68R]), and pie-1::degron::gfp animals (100 µM auxin exposure). Oocyte nuclei are indicated with white dashed circle. (B) Quantification of immunofluorescence intensity in oocytes (−1 to −5). H3K9Ac signal was measured by ImageJ. The mean of the correlated total cell fluorescence (CTCF)/area ± SEM is plotted on the y axis. Significance was measured using a Tukey’s test: ****p<0.0001; *p<0.05. (C and D) Scatter plots comparing mRNA-seq reads in (C) pie-1(ne4303[K68R]) or (D) pie-1::degron::gfp to those in wt. Blue dashed lines indicate twofold increased or decreased in the mutant. Genes were categorized as spermatogenic, oogenic, neutral, or other, as defined by Ortiz et al., 2014. A value of 0.1 was assigned to undetected genes, thus genes with an x value of ‘−1’ were not detected in wt. (E) Bar graph showing fractions of upregulated genes involved in spermatogenesis, oogenesis, neutral, or other categories. Genes expressed in wt gonads were used as a reference (10743 genes) (Kim et al., 2021). The number of upregulated genes in each mutant is labeled at the top. (F) Venn diagram showing overlap of genes upregulated in pie-1::degron::gfp, hda-1[KKRR], and mep-1::degron. The hda-1[KKRR] and mep-1::degron data are from Kim et al., 2021.

Figure 5—source data 1

HDAC immunostaining signal intensities.

https://cdn.elifesciences.org/articles/63300/elife-63300-fig5-data1-v1.xlsx

Acetylation of H3K9 is associated with active transcription (Peterson and Laniel, 2004), and loss of HDA-1 SUMOylation leads to increased transcriptional activity (David et al., 2002). We therefore sequenced mRNAs from dissected pie-1 gonads to determine the extent to which PIE-1 regulates transcription in the adult germline. Whereas pie-1(ne4303[K68R]) gonads exhibited mild changes in mRNA levels (Figure 5C), a group of 479 genes were upregulated by more than twofold in pie-1::degron depleted gonads, as compared to wild type (Figure 5D). Upregulated protein-coding genes, included many spermatogenesis-specific genes (Figure 5E), suggesting that PIE-1 helps ensure a complete transition from spermatogenesis-specific gene expression to oogenesis-specific gene expression in the hermaphrodite. Five transposon families were upregulated (Figure 5—figure supplement 2A), including Tc5 (256-fold) and MIRAGE1 (900-fold), suggesting that PIE-1 activity also promotes transposon silencing in the adult germline. A comparison to adult gonad mRNAs upregulated in MEP-1-depleted animals and in animals homozygous for a putative HDA-1 SUMO acceptor mutant (Kim et al., 2021) revealed a significant overlap, especially among spermatogenesis genes (Figure 5F), suggesting that PIE-1 acts through the NuRD complex to regulate the majority of its adult germline targets.

PIE-1 and GEI-17 act together to promote Piwi Argonaute-mediated silencing

In a parallel study exploring the role of SUMO and NuRD complex co-factors in piRNA-mediated silencing in the germline, we found that mutations in smo-1 and ubc-9 activate germline expression of a piRNA pathway reporter (Kim et al., 2021), but null alleles of gei-17 do not (Figure 6B). We wondered if this failure might reflect a partial redundancy between GEI-17 and PIE-1 in promoting the SUMOylation of targets required for piRNA-directed transcriptional silencing. To test this, we monitored a piRNA sensor for activation in pie-1 and gei-17 single and double mutant strains. As a control, we monitored sensor activation in an rde-3 mutant (Figure 6A), which disrupts the maintenance of silencing downstream in the piRNA pathway (Chen et al., 2005; Gu et al., 2009; Shirayama et al., 2012). The reporter was desilenced in 67% of first-generation rde-3 homozygous worms and reached 100% in third-generation homozygotes (Figure 6B). Two different pie-1 null alleles desilenced the piRNA sensor in 65% (15/23) and 54% (7/13) of first-generation homozygotes, but subsequent generations could not be monitored due to embryo lethality (Figure 6B). The pie-1[K68R] mutation had a mild desilencing effect: the piRNA sensor remained silenced in the first generation, but gradually became active over the next three generations, where it was expressed in ~50% of the fourth-generation homozygotes. Two presumptive gei-17 null alleles failed to desilence the reporter through four generations of monitoring (Figure 6B). While attempting to make the gei-17; pie-1[K68R] double mutant, we found that gei-17/+; pie-1[K68R] hermaphrodites are completely sterile, suggesting that gei-17 is haploinsufficient in pie-1[K68R] mutants. To overcome this problem, we used CRISPR to induce homozygous gei-17 deletion alleles directly in a piRNA sensor strain homozygous for pie-1[K68R]. All 18 gei-17; pie-1[K68R] strains recovered in this way exhibited complete first-generation desilencing of the piRNA sensor (Figure 6B) and were also completely sterile. In contrast, control injections into the otherwise wild-type piRNA sensor strain produced 10 homozygous gei-17 null strains that were fertile and viable but failed to desilence in the piRNA sensor (Figure 6B). Thus PIE-1 and GEI-17 appear to function redundantly to promote piRNA surveillance and fertility in the adult germline.

Figure 6
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PIE-1 and GEI-17 function together to promote piRNA-mediated silencing.

(A) Epifluorescence images (upper panels) of piRNA sensor expression in dissected gonads from wild-type and rde-3(ne3370) worms. The lower panels show differential interference contrast images of the gonads in the upper panels. (B) Synergistic effects of desilencing piRNA sensors in pie-1[K68R]; gei-17 double mutants. The desilenced piRNA sensor (gfp::csr-1) was scored in the indicated alleles. gei-17(null) alleles were generated by CRISPR editing.

Discussion

The PIE-1 protein was originally identified as a maternally provided factor required to prevent early germline cells of the C. elegans embryo from adopting somatic differentiation programs. The PIE-1 protein was found to localize prominently to embryo germline nuclei (Mello et al., 1996), where it was proposed to inhibit pol II activity (Seydoux and Dunn, 1997; Seydoux and Fire, 1994), possibly through direct inhibition of the CTD kinase (Batchelder et al., 1999; Ghosh and Seydoux, 2008). Here, we have shown that PIE-1 is also expressed in the adult germline where it does not directly inhibit transcription, but rather functions along with components of the SUMO pathway to promote the hypoacetylation of germline chromatin and with the SUMO E3 homolog GEI-17 to promote Piwi Argonuate-dependent gene silencing. Although PIE-1 is not SUMOylated in the embryo, our genetic studies indicate that SUMO components, including the SUMO E3 ligase homolog GEI-17, function together with PIE-1 to preserve embryonic germline fates. PIE-1 interacts with SMO-1/SUMO and UBC-9, as well as GEI-17, by yeast two-hybrid, suggesting that PIE-1 may recruit these factors directly to its germline targets. Thus, our findings suggest how PIE-1, through its association with the SUMO pathway, may exert its remarkable dual effects as a germline determinant that controls both transcription and chromatin remodeling.

Using an affinity-based approach and mass spectrometry, we identified hundreds of C. elegans proteins likely to be direct SUMO conjugates. Our results complement published work identifying SUMO-regulated targets in C. elegans (Drabikowski et al., 2018; Kaminsky et al., 2009) and suggest that many SUMOylation substrates remain to be identified (Figure 1—figure supplement 2D and Supplementary file 3). In addition, we have shown that a HIS10::SUMO fusion expressed from the endogenous smo-1 locus is fully functional and can be used along with mutagenesis studies to identify specific SUMO acceptor lysines in substrate proteins (see also Kim et al., 2021). Using these tools, we have shown that both PIE-1 and the type-1 HDAC, HDA-1, are SUMOylated in the adult germline, and that PIE-1 SUMOylation promotes the assembly of an adult germline NuRD complex.

SUMO as an elusive modulator of protein interactions

We found that SUMO modifications to worm target proteins are rapidly and nearly completely reversed in IP sample buffer at 4°C. Consequently, SUMO-dependent protein complexes are likely to rapidly disassemble and to thus be difficult or impossible to detect in co-IP studies. Therefore, the actual in vivo interaction between MEP-1 and HDA-1 in the adult germline may be much more robust than detected here. This possibility is supported by parallel studies in which appending a conjugation-defective SUMO by translational fusion to HDA-1, HDA-1::SMO-1, dramatically increased the association of HDA-1 with MEP-1 and other components of the NuRD complex (Kim et al., 2021). Studies in Drosophila identified a complex, termed MEC, where MEP-1 resides along with Mi-2, but notably, without HDAC (Kunert et al., 2009). The cultured cells where this MEC complex was identified were derived from ovarian tissues and express the Piwi Argonaute (Mugat et al., 2020), raising the question of whether a parallel SUMO-regulated HDAC/MEC complex also functions in the Drosophila ovary but has been missed due to the labile nature of SUMO modifications.

In the embryo HDA-1 is not SUMOylated and yet interacts robustly with its NuRD complex co-factors. We do not know how or why the assembly of HDA-1-NuRD complex differs between embryos and adults. Perhaps, SUMOylation of HDA-1 and other NuRD complex components helps overcome an unknown barrier to co-assembly in the adult germline, enabling the proteins to associate via a mechanism bridged by SUMO (Matunis et al., 2006; Psakhye and Jentsch, 2012; Pelisch et al., 2017). Such a mechanism could render the assembly and function of the adult germline NuRD complex more dynamic and responsive to signals that control the conjugation and removal of SUMO.

PIE-1 as a SUMO E3 and co-factor for the conserved SUMO-E3 GEI-17/PAIS1

Because PIE-1 appears to interact directly with UBC-9, it is possible that PIE-1 harnesses the SUMO-conjugating machinery by acting like an E3 SUMO ligase both for itself and for target proteins. SUMOyation of PIE-1 could enhance its E3 activity and its association with UBC-9 via the non-covalent SUMO-binding site on the backside of UBC-9 (Capili and Lima, 2007a). The N-terminal two-thirds of PIE-1—which includes lysine 68 and both zinc finger motifs—interacts with UBC-9 in our yeast two-hybrid assays (data not shown), and the non-overlapping proline-rich C-terminal domain of PIE-1 interacts with MEP-1 (Unhavaithaya et al., 2002). Thus, PIE-1 may bind UBC-9 and MEP-1 simultaneously. Perhaps this ternary complex transiently associates with HDA-1 to promote its SUMOylation. HDA-1-SUMO might then associate with one or both of the putative SUMO-interacting motifs on MEP-1 (Kim et al., 2021).

A recent study identified the Drosophila GEI-17 homolog Su(var)2–10 as a bridge between a nuclear Piwi Argonaute and a chromatin remodeling complex that includes the histone methyltransferase SetDB1/Eggless (Egg) (Ninova et al., 2020). Our findings raise the possibility that, in addition to SetDB1, the Drosophila Piwi Su(var)2–10 complex may promote SUMOylation of HDAC1 to assemble a germline NuRD complex that prepares chromatin for SetDB1-dependent methylation. Perhaps in animal germlines, SUMO-dependent assembly of the NuRD complex frees it from other tasks, thereby enabling nuclear Argonautes—via associations with SUMO E3 enzymes—to recruit and assemble this vital chromatin remodeling and silencing machinery at their targets.

Materials and methods

Key resources table
Reagent type
(species) or
resource		DesignationSource or
reference		IdentifiersAdditional
information
AntibodyMouse monoclonal anti-FLAG M2Sigma-AldrichCat# F1804; RRID:AB_262044IB(1:1000)
AntibodyRabbit polyclonal anti-MRG-1Novus BiologicalsCat# 49130002; RRID:AB_10011724IB(1:1000)
AntibodyRabbit polyclonal anti-HDA-1Novus BiologicalsCat# 38660002;
RRID:AB_10708816		IB(1:2500)
AntibodyRabbit polyclonal anti-LET-418Novus BiologicalsCat# 48960002; RRID:AB_10708820IB(1:1000)
AntibodyRat monoclonal anti-tubulinBio-RadCat# MCA77G; RRID:AB_325003IB(1:2000)
AntibodyMouse monoclonal anti-histone H3, acetyl K9AbcamCat# ab12179; RRID:AB_298910IF(1:100)
AntibodyRabbit polyclonal anti-PRG-1Batista et al., 2008N/AIB(1:1000)
AntibodyMouse monoclonal anti-SMO-1Pelisch et al., 2017Gift from Hay LabIB(1:500)
Freshly purified from hybridoma cell culture
AntibodyMouse monoclonal anti-PIE-1(P4G5)Mello et al., 1996N/AIB(1:100)
AntibodyGoat anti-mouse IgG (HRP-conjugated)Thermo Fisher ScientificCat# 62–6520; RRID:AB_2533947IB(1:2500)
AntibodyMouse anti-rabbit IgG light (HRP-conjugated)AbcamCat# ab99697; RRID:AB_10673897IB(1:3000)
AntibodyAnti-rat IgG (HRP-conjugated)Jackson ImmunoResearch LabsCat# 712-035-150; RRID:AB_2340638IB(1:5000)
AntibodyGoat anti-mouse IgG (H + L) Alexa Fluor 594Thermo Fisher Scientific(Cat# A-11005; RRID:AB_2534073)IF(1:1000)
Strain, strain backgroundC. elegans strainsThis studySupplementary file 5
Strain, strain backgroundE. coli: strain OP50Caenorhabditis Genetics CenterWormBase: OP50
Strain, strain backgroundE. coli: strain HT115Caenorhabditis Genetics CenterWormBase: HT115
Strain, strain backgroundE. coli: Ahringer collectionLaboratory of C. MelloN/A
Peptide,
recombinant protein		Ex Taq DNA polymeraseTakaraCat# RR001C
Peptide,
recombinant protein		iProof high fidelity DNA polymeraseBio-RadCat#1725302
Peptide,
recombinant protein		BsaINew England BiolabsCat# R3535S
Peptide,
recombinant protein		NheINew England
Biolabs		Cat# R3131S
Peptide,
recombinant protein		HaeIII (screen for G56R)New England BiolabsCat# R0108S
Peptide,
recombinant protein		Alt-R S.p. Cas9 Nuclease V3Integrated DNA Technologies (IDT)Cat# 1081058CRISPR reagent
Peptide,
recombinant protein		GFP-binding protein beadsHomemadeN/A
Chemical compound, drugIsopropyl-β-D-thiogalactosideSigma-AldrichCat# 11411446001
Chemical compound, drugAmpicillinSigma-AldrichCat# A9518
Chemical compound, drugTetracyclineSigma-AldrichCat# 87128
Chemical compound, drugIndole-3-acetic acidAlfa AesarCat# A10556
Chemical compound, drugTetramisole hydrochlorideSigma-AldrichCat# L9756-5G
Chemical compound, drugParaformaldehyde 16% solutionElectron Microscopy ScienceCat# Nm15710
Chemical compound, drugPBSLife TechnologiesCat# AM9615
Chemical compound, drugTween20Fisher BioReagentsCat# BP337-500
Chemical compound, drugBovine serum albuminLife TechnologiesCat# AM2618
Chemical compound, drug1M HEPES, pH 7.4TEKnovaCat# H1030
Chemical compound, drugSodium citrate dihydrateThermo Fisher ScientificCat# BP337500
Chemical compound, drugTriton X-100Sigma-AldrichCat# T8787-250ml
Chemical compound, drugComplete EDTA-freeprotease inhibitor cocktailRocheCat# 11836170001
Chemical compound, drugNP-40EMD MilliporeCat# 492018
Chemical compound, drugTris (Base)AvantorCat# 4099–06
Chemical compound, drugBoric acidAMRESCOCat# M139
Chemical compound, drugEthylenediaminetetraacetic acid disodium salt dihydrateSigma-AldrichCat# E1644
Chemical compound, drugSodium dodecyl sulfateSigma-AldrichCat# L3771-100G
Chemical compound, drugSodium chlorideGenesee ScientificCat# 18–214
Chemical compound, drugMagnesium chlorideSigma-AldrichCat# M8266
Chemical compound, drugDL-dithiothreitolSigma-AldrichCat# D0632-10G
Chemical compound, drugPotassium acetateFisher BioReagentsCat# BP364-500
Chemical compound, drugAmmonium acetateSigma-AldrichCat# A7262
Chemical compound, drugDeoxy-bigCHAPAlfa AesarCat# J64578-MD
Chemical compound, drugPotassium chlorideSigma-AldrichCat# P9541
Chemical compound, drugGuanidine-HClSigma-AldrichCat# G3272
Chemical compound, drugImidazoleSigma-AldrichCat# 792527
Chemical compound, drugβ-MercaptoethanolSigma-AldrichCat# M6250
Chemical compound, drugSodium phosphate, dibasicSigma-AldrichCat# S7907
Chemical compound, drugSodium phosphate, monobasicSigma-AldrichCat# S0751
Chemical compound, drugUreaThermo Fisher ScientificCat# Ac327380010
Chemical compound, drugTrichloroacetic acidSigma-AldrichCat# T0699
Chemical compound, drug1-Bromo-3-chloropropaneSigma-AldrichCat# B9673
Chemical compound, drugTE buffer, pH 8.0Thermo Fisher ScientificCat# AM9858
Chemical compound, drugTris(2-carboxyethyl)phosphine hydrochlorideSigma-AldrichCat# C4706
Chemical compound, drugTrypsinNew England BiolabsCat# P8101S
Chemical compound, drugTRI reagentSigma-AldrichCat# T9424
Chemical compound, drugIodoacetamideSigma-AldrichCat# I1149
Commercial assay, kitNi-NTA resinQiagenCat# 30210
Commercial assay, kitSlowFade Diamond antifade Mountant with DAPILife TechnologiesCat# S36964
Commercial assay, kitQuick start Bradford 1× dye reagentBio-RadCat# 5000205
Commercial assay, kitGlycoBlueCoprecipitantThermo Fisher ScientificCat# AM9515
Commercial assay, kitNuPage LDS sample buffer (4×)Thermo Fisher ScientificCat# NP0008
Commercial assay, kitpCR-Blunt II-TOPO cloning kitThermo Fisher ScientificCat# K280020
Commercial assay, kitPierce Silver Stain KitThermo Fisher ScientificCat# 24612
Commercial assay, kitLumi-Light Plus western blotting substrateSigma-AldrichCat# 12015196001
Commercial assay, kitHyperfilm ECLThermo Fisher ScientificCat# 45001507
Commercial assay, kitKAPA RNA HyperPrep with RiboErase (KK8560)RocheCat# 08098131702
Commercial assay, kitKAPA single-indexed adapter kit (KK8700)RocheCat# 08005699001
Commercial assay, kitIllumina NextSeq 500/550 v2.5 kit (150 cycles)IlluminaCat# 20024907
Recombinant DNA reagentPeft3::cas9 vector (backbone: blunt II topo vector in this study)Friedland et al., 2013N/ABackbone is changed to blunt II topo vector in this study
Recombinant DNA reagentpRF4: injection marker, rol-6(su1006)Mello et al., 1991N/ABackbone is changed to blunt II topo vector in this study
Recombinant DNA reagentsgRNA plasmidThis studySee Materials and methods; Supplementary file 6
Sequence-based reagentgRNA and ss oligo donor sequencesThis studySupplementary file 6
Sequence-based reagentAlt-R CRISPR-Cas9 tracrRNAIntegrated DNA Technologies (IDT)Cat# 1072534CRISPR reagent
Software, algorithmGraphPad Prism version 8.2.1GraphPad Softwarehttp://www.graphpad.com
Software, algorithmImageJRueden et al., 2017https://imagej.net
Software, algorithmStrata 15.1Strata Statistical Softwarehttp://www.strata.com
Software, algorithmSalmonPatro et al., 2017Version 1.1.0
Software, algorithmDESeq2Love et al., 2014Version 1.26.0
Software, algorithmProlucidXu et al., 2006N/A
Software, algorithmDTASelect 2Tabb et al., 2002N/A

C. elegans strains and genetics

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Strains and alleles used in this study were listed in Supplementary file 5. Worms were, unless otherwise stated, cultured at 20°C on NGM plates seeded with OP50 Escherichia coli, and genetic analyses were performed essentially as described (Brenner, 1974).

CRISPR/Cas9 genome editing

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The Co-CRISPR strategy (Kim et al., 2014) using unc-22 sgRNA as a co-CRISPR marker was used to enrich HR events for tagging a gene of interest with the non-visualizing epitope (6xhis and 10xhis) or introduction of a point mutation (G56R). To screen for insertions of 6xhis and 10xhis, we used two-round PCR: the first PCR was performed with primers (F: cctcaaaaaccaagcgaaaacc R: ccggctgctatttcattgat), and 1 µl of the first PCR product was used as a template for the second PCR with primers (F:gagactcccgctataaacga R:ctcaagcaggcgacaacgcc). To detect 6xhis or 10xhis knock-ins, the final products were run either on 2% Tris/borate/EDTA (TBE) gel or 10% PAGE gel. The ubc-9(G56R) mutation introduced an HaeIII restriction fragment length polymorphisms (RFLP) that was used to screen for G56R conversion in PCR products (F: cattacatggcaagtcggg, R: cgttgccgcatacagaaatag). For visualization of either GFP tag, F1 rollers were mounted under coverslips on 2% agarose pads to directly screen for GFP expressing animals as described previously (Kim et al., 2014). 3xflag knock-ins to pie-1(ne4303) were screened by PCR using previously reported primers (Kim et al., 2014).

sgRNA construct: Previously generated pie-1 sgRNA plasmid (Kim et al., 2014) was used for pie-1::degron::gfp and pie-1(K68R)::flag. Others were constructed by ligating annealed sgRNA oligonucleotides to Bsal-cut pRB1017 (Arribere et al., 2014) and sgRNA sequences are listed in Supplementary file 6.

Donor template: Unless otherwise stated, a silent mutation to disrupt the PAM site in each HR donor was introduced by PCR sewing.

ubc-9(G56R): For the ubc-9(G56R) donor construct, a ubc-9 fragment was amplified with primers (F: cattacatggcaagtcggg, R: gacgactaccacgaagcaagc) and this fragment was cloned into the Blunt II-TOPO vector (Thermo Fisher Scientific, K2800-20). To introduce the point mutation (G56R) and mutate the seeding region, overlap extension PCR was used.

6xhis::smo-1/10xhis::smo-1: Using PCR sewing, either 6xhis (caccatcaccaccatcac) or 10xhis fragment (caccatcaccatcaccatcaccaccatcac) was introduced immediately after the start codon in the previously generated smo-1 fragment (Kim et al., 2014). The resulting PCR product was cloned into the Blunt II-TOPO vector. Tagging with his tag on the N-terminus of smo-1 disrupted the PAM site.

mep-1::gfp::tev::3xflag: For the mep-1::gfp::tev::3xflag donor construct, a mep-1 fragment was amplified with primers (F1:gaaattcgctggcagtttct R1: ctgcaacttcgatcaatcga) from N2 genomic DNA and inserted into the pCR-Blunt II-TOPO vector. Overlap extension PCR was used to introduce a NheI site immediately before the stop codon in this mep-1 fragment. The NheI site was used to insert the gfp::tev::3xflag coding sequence.

pie-1(K68R)::3xflag and pie-1::degron::gfp: A previously generated donor plasmid (Kim et al., 2014) was used for pie-1(K68R)::3xflag. For pie-1::degron::gfp donor construct, a degron coding sequence with flanking NheI sites was amplified from pLZ29 plasmid (Zhang et al., 2015) and cloned the NheI fragment into a unique NheI sitee in the pie-1::gfp plasmid (Kim et al., 2014).

Other mutant alleles of pie-1, gei-17, and rde-3 were generated by editing using Cas9 ribonucleoprotein (Dokshin et al., 2018). Guide RNA sequences and ssOligo donor sequence are listed in Supplementary file 6.

Yeast two-hybrid analysis

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The yeast two-hybrid screen was performed by Hybrigenics Services (Paris, France, http://www.hybrigenics-services.com). The coding sequence for amino acids 2–335 of C. elegans pie-1 (NM_001268237.1) was amplified by PCR from N2 cDNA and cloned into pB66 downstream of the Gal4 DNA-binding domain sequence. The construct was sequenced and used as a bait to screen a random-primed C. elegans mixed-stage cDNA library in the pP6 plasmid backbone (which encodes the Gal4 activation domain). The library was screened using a mating approach with YHGX13 (Y187 ade2-101::loxp-kanMX-loxP, matα) and CG1945 (mata) yeast strains as previously described (Fromont-Racine et al., 1997). Five-million colonies—i.e., five times the complexity of the library—were screened. 153 His+ colonies were selected on medium lacking tryptophan, leucine, and histidine, and supplemented with 0.5 mM 3-aminotriazole to prevent bait autoactivation. The prey fragments of the positive clones were amplified by PCR and sequenced at their 5’ and 3’ junctions to identify the corresponding interacting proteins in the GenBank database (NCBI) using a fully automated procedure. A confidence score (predicted biological score) was attributed to each interaction as previously described (Formstecher et al., 2005).

Auxin treatment

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The pie-1::degron::gfp sequence was inserted into the endogenous pie-1 gene in CA1199 (unc-119(ed3); ieSi38 [Psun-1::TIR1::mRuby::sun-1 3’UTR, cb-unc-119(+)] IV) (Zhang et al., 2015) by CRISPR/Cas9-mediated genome editing. The degron-tagged L1 larvae worms were plated on NGM plates containing 100 µM auxin indole-3-acetic acid (Alfa Aesar, A10556). Worms were collected for gonad dissection when the population reached the adult stage.

RNAi

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RNAi was performed by feeding worms E. coli HT115 (DE3) transformed with control (empty) vector or a gene-targeting construct from the C. elegans RNAi collection (Kamath and Ahringer, 2003). For the genetic analysis, L4 larvae were placed on NGM plates containing 1 mM isopropyl β-D-thiogalactoside (IPTG) and 100 µg/ml ampicillin seeded with control or RNAi bacteria. After 24 hr, adult worms were transferred to fresh RNAi plates and allowed to lay eggs overnight. The following day, adults were removed from the test plates, and unhatched eggs were analyzed 12 hr later. For biochemical assays, ~200,000 synchronous L4 worms were placed on RNAi plates containing 0.4 mM IPTG, 100 µg/ml ampicillin, and 12.5 µg/ml tetracycline.

Immunofluorescence

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Gonads were dissected on a glass slide (Thermo Fisher Scientific, 1256820) in egg buffer (25 mM HEPES pH 7.5, 118 mM NaCl, 48 mM KCl, 2 mM CaCl2, 2 mM MgCl2) containing 0.2 mM tetramisole (Sigma-Aldrich, L9756). The samples were transferred into a Slickseal microcentrifuge tube (National Scientific, CA170S-BP) and fixed with 2% paraformaldehyde (Electron Microscopy Science, Nm15710) in phosphate-buffered saline (PBS) pH 7.4 for 10 min, and –20°C cold 100% methanol for 5 min. Fixed samples were washed four times with PBST (PBS containing 0.1% Tween20) containing 0.1% bovine serum albumin (BSA), blocked in PBST containing 1% BSA for 1 hr, and then incubated overnight at 4°C with anti-histone H3 acetyl-K9 (Abcam, ab12179) diluted 1:100 in PBST containing 1% BSA. After four washes with PBST containing 0.1% BSA, samples were incubated for 2 hr at room temperature with goat anti-mouse IgG (H + L) Alexa Fluor 594 (Thermo Fisher Scientific, A-11005) diluted 1:1000 in PBST containing 1% BSA. Samples were washed four times with PBST containing 0.1% BSA, transferred to poly-L-lysine coated slides (LabScientific, 7799) and mounted with 10 µl of SlowFade Diamond Antifade Mountant with DAPI (Life Technologies, S36964).

Microscopy

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For live imaging, worms and embryos were mounted in M9 on a 2% agarose pad with or without 1 mM tetramisole. Epifluorescence and differential interference contrast microscopy were performed using an Axio Imager M2 Microscope (Zeiss). Images were captured with an ORCA-ER digital camera (Hamamatsu) and processed using Axiovision software (Zeiss). Confocal images were acquired using a Zeiss Axiover 200 M microscope equipped with a Yokogawa CSU21 spinning disk confocal scan head and custom laser launch and relay optics (Solamere Technology Group). Stacks of images were taken and analyzed using ImageJ.

Immunoprecipitation

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Either synchronous adult worms (~200,000) or early embryos (from 10 plates of 100,000 adults) were collected, washed three times with M9 buffer, suspended in lysis buffer composed of 20 mM HEPES (pH 7.5), 125 mM sodium citrate, 0.1% (v/v) Tween 20, 0.5% (v/v) Triton X-100, 2 mM MgCl2, 1 mM DTT, and a Mini Protease Inhibitor Cocktail Tablet (Roche), and homogenized in a FastPrep-24 benchtop homogenizer (MP Biomedicals). Worm or embryo lysates were centrifuged twice at 14,000 × g for 30 min at 4°C, and supernatants were incubated with GBP beads for 1.5 hr at 4°C on a rotating shaker. The beads were washed three times with IP buffer containing protease inhibitor for 5 min each wash, and then washed twice with high-salt wash buffer (50 mM HEPES pH 7.5, 500 mM KCl, 0.05% NP40, 0.5 mM DTT, and protease inhibitor). Immune complexes were eluted with elution buffer (50 mM Tris-HCl pH 8.0, 1× SDS) for 10 min at 95°C.

Affinity chromatography of histidine-tagged SUMO

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Synchronous adult worms (~200,000) or 500 µl of packed embryos (from ~1,000,000 synchronous adult worms) were homogenized in lysis buffer at pH 8.0 (6 M guanidine-HCl, 100 mM Na2HPO4/NaH2PO4 pH 8.0, and 10 mM Tris-HCl pH 8.0) using a FastPrep-24 benchtop homogenizer (MP Biomedicals). Lysates were cleared by centrifugation at 14,000 × g for 30 min at 4°C and quantified using the Quick Start Bradford 1 × Dye Reagent (BioRad, 5000205). Ni-NTA resin was washed three times with lysis buffer containing 20 mM imidazole pH 8.0 and 5 mM β-mercaptoethanol while samples were prepared. To equalized samples, we added imidazole pH 8.0 to 20 mM and β-mercaptoethanol to 5 mM, and then the samples were incubated with 100 µl of pre-cleared 50% slurry of Ni-NTA resin (Qiagen, 30210) for 2–3 hr at room temperature on a rotating shaker. Ni-NTA resin was washed in 1 ml aliquots of the following series of buffers: Buffer 1 pH 8.0 (6 M guanidine-HCl, 100 mM Na2HPO4/NaH2PO4 pH 8.0, 10 mM Tris-HCl pH 8.0, 10 mM imidazole pH 8.0, 5 mM β-mercaptoethanol, and 0.1% Triton X-100), Buffer 2 pH 8.0 (8 M urea, 100 mM Na2HPO4/NaH2PO4 pH 8.0, 10 mM Tris-HCl pH 8.0, 10 mM imidazole pH 8.0, 5 mM β-mercaptoethanol, and 0.1% Triton X-100), Buffer 3 pH 7.0 (8 M urea, 100 mM Na2HPO4/NaH2PO4 pH 7.0, 10 mM Tris-HCl pH 7.0, 10 mM imidazole pH 7.0, 5 mM β-mercaptoethanol, and 0.1% Triton X-100), Buffer 4 pH 6.3 (8 M urea, 100 mM Na2HPO4/NaH2PO4 pH 6.3, 10 mM Tris-HCl pH 6.3, 10 mM imidazole pH 6.3, 5 mM β-mercaptoethanol, and 0.1% Triton X-100), Buffer 5 pH 6.3 (8 M urea, 100 mM Na2HPO4/NaH2PO4 pH 6.3, 10 mM Tris-HCl pH 6.3, and 5 mM β-mercaptoethanol). Urea was used to denature proteins. Triton-X-100, the non-ionic detergent, was used to reduce nonspecific hydrophobic interactions. Imidazole (10 mM) was used to increase the stringency of the wash by reducing nonspecific protein binding to the resin. The use of wash buffers with gradually decreasing pH (pH 8-6.3) also reduced nonspecific binding of proteins by protonating the neutral histidine and thereby removing the weakly bound proteins that may contain tandem repeats of the histidine. SUMOylated proteins were eluted with elution buffer pH 7.0 (7 M urea, 100 mM Na2HPO4/NaH2PO4 pH 7.0, 10 mM Tris-HCl pH 7.0, and 500 mM imidazole pH 7.0). For western blotting, input samples containing guanidine-HCl were diluted with H2O (1:6) and then purified by trichloroacetic acid (TCA) precipitation: an equal volume of 10% TCA was added to diluted samples, which were then incubated on ice for 20 min and centrifuged for 20 min at 4°C; the obtained pellet was washed with 100 µl of ice-cold ethanol and then resuspended in Tris-HCl buffer pH 8.0.

Western blot analysis

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NuPAGE LDS sample buffer (4×) (Thermo Fisher Scientific, NP0008) was added to samples, which were then loaded on precast NuPAGE Novex 4–12% Bis-Tris protein gel (Life Technologies, NP0321BOX) and transferred onto a polyvinylidene difluoride membrane (Bio-Rad Laboratories, 1704157) using Mini Trans-Blot cells (Bio-Rad Laboratories, 1703930) at 80 V for 2.2 hr, at 4°C. Membranes were blocked with 5% (w/v) skim milk in PBST and probed with primary antibodies: 1:1000 anti-FLAG (Sigma-Aldrich, F1804); 1:1000 anti-MRG-1 (Novus Biologicals, 49130002); 1:2500 anti-HDA-1 (Novus Biologicals, 38660002); 1:1000 anti-LET-418 (Novus Biologicals, 48960002); 1:1000anti-SMO-1 (purified from Hybridoma cell cultures; the Hybridoma cell line was a gift from Ronald T. Hay, University of Dundee) (Pelisch et al., 2017); 1:2000 anti-tubulin (Bio-Rad, MCA77G); 1:100 anti-PIE-1(P4G5); or 1:1000 anti-PRG-1. Antibody binding was detected with secondary antibodies: 1:2500 goat anti-mouse (Thermo Fisher Scientific, 62–6520); 1:3000 mouse anti-rabbit (Abcam, ab99697); 1:5000 anti-rat (Jackson ImmunoResearch Labs, 712-035-150).

RNA-seq

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Germline RNA was extracted from 100 dissected gonads using TRI reagent (Sigma-Aldrich, T9424). Total RNA (500 ng per replica) was used for library construction using KAPA RNA HyperPrep with RiboErase (Kapa Biosystems, KK8560) and KAPA single-indexed adapter (Kapa Biosystems, KK8700) for Illumina platforms. Paired-end sequencing was performed on a NextSeq 500 Sequencer with Illumina NextSeq 500/550 high output kit v2.5 (150 cycles) (Illumina, 20024907). Salmon was used to map and quantify the reads against the worm database WS268, and its output files were imported to DESeq2 in R. Differentially expressed genes were defined as twofold change and adjusted p-value less than 0.05 (Supplementary file 7). The scatter plots were generated by the plot function in R. Comparisons between repeats of each sample are in Figure 5—figure supplement 2B.

SUMO proteomics

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HIS10::SMO-1 samples (or control samples) precipitated from adult lysates were solubilized in 8 M urea, 100 mM Tris (pH 8.0), reduced in 5 mM TCEP for 20 min, alkylated with 10 mM iodoacetamide for 15 min, and digested with trypsin. Each fraction was analyzed on a Q Exactive HF mass spectrometer (Thermo Fisher Scientific) coupled to a nano UHPLC Easy-nLC 1000 via a nano-electrospray ion source. Peptides were separated on a home-packed capillary reverse phase column (75 μm internal diameter × 15 cm of 1.8 μm, 120 Å UHPLC-XB-C18 resin) with a 110 min gradient of A and B buffers (buffer A, 0.1% formic acid; buffer B, 100% ACN/0.1% formic acid). A lock mass of 445.120025 m/z was used for internal calibration. Electrospray ionization was carried out at 2.0 kV, with the heated capillary temperature set to 275°C. Full-scan mass spectra were obtained in the positive-ion mode over the m/z range of 300–2000 at a resolution of 120,000. MS/MS spectra were acquired in the Orbitrap for the 15 most abundant multiply charged species in the full-scan spectrum having signal intensities of >1 × 10−5 NL at a resolution of 15,000. Dynamic exclusion was set such that MS/MS was acquired only once for each species over a period of 30 s. The MS data was searched against the concatenated forward and reversed C. elegans protein database (WS233) using by Prolucid (Xu et al., 2006) and DTASelect 2 (Tabb et al., 2002) (≤1% false discovery rate at the peptide level).

Data availability

RNA sequencing data have been deposited in NCBI under accession codes SRR12454798 to 12454800 and are included in Supplementary file. All data generated or analyzed during this study are included in the manuscript and supplementary files.

The following data sets were generated
    1. Mello CC
    (2021) NCBI BioProject
    ID PRJNA657260. Gonad mRNA sequencing of pie-1 mutant in C. elegans.
    https://www.ncbi.nlm.nih.gov/bioproject/PRJNA657260

References

  6. Book
    1. Blackshear PJ
    2. Phillips RS
    3. Lai WS
    (2005) Tandem CCCH Zinc Finger Proteins in mRNA Binding
    In: Iuchi S, Kuldell N, editors. Zinc Finger Proteins. Molecular Biology Intelligence Unit. Boston: Springer. pp. 80–90.
    https://doi.org/10.1007/0-387-27421-9_13
    1. Brenner S
    (1974)
    The genetics of Caenorhabditis elegans
    Genetics 77:71–94.

Decision letter

  1. Tony Hunter
    Reviewing Editor; Salk Institute for Biological Studies, United States
  2. Kevin Struhl
    Senior Editor; Harvard Medical School, United States
  3. Tony Hunter
    Reviewer; Salk Institute for Biological Studies, United States
  4. Federico Pelisch
    Reviewer; University of Dundee, United Kingdom

In the interests of transparency, eLife publishes the most substantive revision requests and the accompanying author responses.

Acceptance summary:

These studies extend the findings in the accompanying paper, which showed that sumoylation of the HDA-1 type histone deacetylase plays a role in establishing transcriptional silencing of piRNA-regulated genes in C. elegans by promoting local histone deacetylation. Here, the authors provide genetic evidence that the PIE-1 zinc finger protein is important for silencing of piRNA-regulated genes, and show that sumoylation of lysine 68 in the PIE-1 zinc finger protein is required for both for its association with HDA-1 and for sumoylation of HDA-1, demonstrating that PIE-1 sumoylation plays a role in piRNA-mediated silencing of gene expression in C. elegans.

Decision letter after peer review:

Thank you for submitting your article "PIE-1 promotes SUMOylation and activation of HDAC1 during the C. elegans oogenesis" for consideration by eLife. Your article has been reviewed by 3 peer reviewers, including Tony Hunter as the Reviewing Editor and Reviewer #1, and the evaluation has been overseen by Kevin Struhl as the Senior Editor. The following individual involved in review of your submission has agreed to reveal their identity: Federico Pelisch (Reviewer #2).

The reviewers have discussed the reviews with one another and the Reviewing Editor has drafted this decision to help you prepare a revised submission.

As the editors have judged that your manuscript is of interest, but as described below that additional experiments are required before it is published, we would like to draw your attention to changes in our revision policy that we have made in response to COVID-19 (https://elifesciences.org/articles/57162). First, because many researchers have temporarily lost access to the labs, we will give authors as much time as they need to submit revised manuscripts. We are also offering, if you choose, to post the manuscript to bioRxiv (if it is not already there) along with this decision letter and a formal designation that the manuscript is "in revision at eLife". Please let us know if you would like to pursue this option. (If your work is more suitable for medRxiv, you will need to post the preprint yourself, as the mechanisms for us to do so are still in development.)

Summary:

In this paper you describe experiments showing that PIE-1 is sumoylated at K68, and that K68 sumoylation plays a role in PIE-1 interaction with HDA-1 and its sumoylation, which leads to its activation. The reviewers found the sumoylation dependence of PIE-1 function in piRNA silencing to be of interest, but raised major issues that need to be addressed. In particular, more mechanistic insights into how sumoylation of PIE-1 at K68 enhances HDA-1 sumoylation and regulation are required

Essential revisions:

1. How sumoylation of K68 affects PIE-1 function, the nature of the SUMO E3 ligase that sumoylates PIE-1, whether sumoylated PIE-1 interacts directly with HDA-1, and, and if so, whether this requires interaction of the K68 SUMO moiety with HDA-1 (e.g. via a SIM) were not elucidated, and need to be addressed with new experimental data. For instance, does a SUMO::K68R PIE-1 fusion complement the pie-1 mutant, or is the exact site of PIE-1 sumoylation important? Also, in vitro deacetylase assays of the sort suggested in the decision letter for eLife-63299, are needed to determine if PIE-1 K68 sumoylation leads to increased HDA-1 enzymatic activity by comparing WT and K68R PIE-1 strains. Additional suggestions for investigating the interaction of PIE-1 with HDA-1 and UBC-9 can be found in Reviewer 1's point 1.

2. Additional supporting data, including in vitro experiments (and better controlled immunoblot exposures) are needed to prove that PIE-1 sumoylation is important for interactions between HDA-1 and PIE-1, UBC-9 and MEP-1. The current data are not convincing.

Additional points are raised in the individual reviews and could be addressed, if the authors believe that addressing them would strengthen the manuscript.

Reviewer #1:

The evidence that sumoylation of K68 in the PIE-1 zinc finger protein is important for HDA-1 type 1 histone deacetylase association and sumoylation seems reasonable, and, is important because as shown in the co-submitted paper HDA-1 sumoylation leads to its association with MEP-1 and LET-418/NuRD complex thus accelerating H3K9ac deacetylation, and silencing gene expression..

The evidence that PIE-1 is needed for sumoylation of HDA-1, presumably though association of PIE-1 with the UBC-9 SUMO E2, is reasonable. However, several aspects of the authors' model remain unclear, and there is an absence of biochemical assays to establish the role of sumoylated PIE-1 in HDA-1 sumoylation, and the effects of sumoylation on HDA-1 HDAC activity.

1. How sumoylation of K68 in PIE1 affects its function was not worked out. Can the deleterious effect of the K68R mutation on PIE-1 function be reversed by generating a SUMO-PIE-1 fusion, as was done for HDA-1 in the co-submitted paper? K68 maps to the N-terminal side of ZF1 in the PIE-1 protein in what appears to be an unstructured region. Does the SUMO residue play a role in the interaction of PIE-1 with HDA-1? Are the zinc fingers required for PIE-1 interaction with HDA-1 or UBC-9? No zinc finger mutations were tested. Does HDA-1 have a SIM that would allow it to interact selectively with sumoylated PIE-1? Another, possibility is that the PIE-1 SUMO moiety is important because it interacts with the non-covalent SUMO-binding site on the backside of UBC-9 (Capill and Lima, JMB 369:606, 2007), which might stabilize the interaction. The backside interaction of SUMO with UBC-9 is proposed to promote UBC-9-mediated sumoylation of target proteins with SUMO consensus sites that are directly recognized by UBC-9. In this scenario, SUMO-PIE-1 would in effect be acting as an E3 SUMO ligase for HDA-1 by serving as a recruitment "factor". In this regard, the authors could test biochemically whether recombinant PIE-1 or K68SUMO-PIE-1 stimulates sumoylation of HDA-1 by UBC-9, using recombinant WT and KKRR mutant HDA-1 as substrates. These issues deserve discussion.

2. What is the SUMO E3 ligase that sumoylates PIE-1? Is it possible that through association with UBC-9, perhaps through its zinc fingers, PIE-1 is sumoylated in cis within a PIE-1/UBC-9 complex?

3. In many places, including the title, the authors make the claim that PIE-1 promotes sumoylation and activation of HDA-1. While it is clear that PIE-1 does increase sumoylation of HDA-1, in a manner requiring K68, and that H3K9ac levels are decreased as a result, the authors do not provide any direct evidence that this process increases HDA-1 catalytic activity, as is implied in the title and elsewhere. As indicated in the review of the co-submitted paper, this would need to be established by carrying out an HDAC assay on control and sumoylated HDA-1 in vitro. Instead of enzymatic activation, it is possible that the PIE-1 interaction and HDA-1 sumoylation results in relocalization of HDA-1 within the nucleus to facilitate more efficient H3K9ac deacetylation.

Reviewer #2:

In their manuscript, Kim et al. address the role of PIE-1 sumoylation during C. elegans oogenesis. The authors favour a model in which sumoylated PIE-1 acts as a sort of E3-like factor 'enhancing' HDA-1 sumoylation. While the results are indeed very interesting, it is unclear to me whether there is enough data to support the author's model. I have list of comments, suggestions, questions, and concerns, which are listed below, which I hope will help the authors strengthen the manuscript:

Figure 1:

i. As with the accompanying manuscript, the extremely low level of SUMO modification should be factored in the model.

ii. Is sumoylation also observed in untagged pie-1? As juged by figure 3A, the authors have a very good antibody to test this.

iii. While the authors claim that PIE-1 sumoylation is not observed in embryos, that panel show a lower exposure than the corresponding one in Adult (as judged by the co-purified unmodified PIE-1::FLAG). A longer exposure and/or more loading would be helpful.

iv. Their strategy and optimisation for purification of sumoylated proteins is excellent and will be useful for future research (along with other reagents the authors developed here). Is the 10xHis::smo-1 functional? Could this be tested in vitro and/or in vivo?

v. In vitro PIE-1 sumoylation would be a desirable addition to this figure.

vi. In addition to germline PIE-1 localisation, it would be interesting to see embryos and PIE-1(K68R).

vii. MW markers are missing in the blots.

Figure 2:

i. The generation of the ubc-9 ts allele is an exceptional tool. Could the authors show SUMO conjugation levels at permissive vs restrictive temperature? Just out of curiosity, is this a fast-acting allele?

ii. The authors mention that gei-17 alleles are viable, could the authors mention any thoughts on why the tm2723 allele is lethal/sterile?

Figure 3:

i. Panel C is mentioned in the text in the wrong place. Also in C, what do the authors think about the big increase in MEP-1 sumoylation in the PIE-1(K68R) background?

ii. I have the same comment for panel D as I had for figure 1 comment III: the exposure/loading for the embryo WB seems lower, as judged by the co-purifying, unmodified HDA-1. A positive control for sumoylated protein coming from embryos would be nice.

iii. In general, the model of PIE-1 acting as a SUMO machinery recruiter should be tested with recombinant proteins. Even if compatible with some results in vivo, showing that this is a plausible mechanism in vitro would be extremely helpful and greatly support the authors' claim.

Figure 4:

i. The authors make a quantitative comparison of the HDA-1/MEP-1 interaction in the text. I think this is not correct. Even if these have been run in the same gel, this could just be a lower exposure. In this line, the HDA-1 blot in the 'Adult' IP would benefit from a longer exposure to better appreciate what seems a rather small difference between PIE-1 and PIE-1(K68R).

ii. Since there still seems to be interaction between MEP-1 and HDA-1 in the PIE-1(K68R) background, does smo-1(RNAi) or ubc-9(G56R) reduce this further?

iii. In panel B, the LET-418 blot on the right is massively overexposed.

iv. Once again, in vitro binding experiments to get some indication that the authors' model is plausible would be a great addition.

Figure 5:

i. Could the authors make some quantitation of the immunofluorescence data?

Overall, I think this manuscript proposes a very interesting model and the results support this model, although I am not convinced these are sufficient to strongly back the authors' claims. I would very much like to see a revised version with some in vitro data backing the authors' model.

Reviewer #3:

In the manuscript by Kim et al., show that, beyond its roles of preventing somatic differentiation in the germline of embryos, Zn-finger protein PIE-1 also functions in the adult germline, where it is both SUMOylated as well as interacts with the SUMO conjugating machinery and promotes SUMOylation of protein targets. They identify HDA-1 as a target of PIE-1-induced SUMOylation. Here too, I find the claims interesting, however data is sometimes missing or does not fully support the claims.

1. A key claim of novelty over previously proposed "glue" functions of SUMO is based on the fact that they find that temporally regulated SUMOylation of a very specific residue in a specific protein is affecting protein activity: The observation that "SUMOylation of HDA-1 only appears to regulate its functions in the adult germline" and not in the embryo together with the finding that "other co-factors such as MEP-1 are SUMOylated more broadly, these findings imply that SUMOylation in the context of these chromatin remodeling complexes, does not merely function as a SUMO-glue (Matunis et al., 2006) but rather has specificity depending on which components of the complex are modified and/or when."

I find this claim poorly supported by the data. In fact, I find that the data supports that multiple SUMOylations contribute to formation of larger complexes: The His-SUMO IP (Figure 2B) brings down far more un-SUMOylated HDA-1 than SUMOylated. This argues for the presence of large complexes with different factors being SUMOylated and many bringing down unmodified HDA-1. The chromatography experiments (Figure 3B-C) also provide hits that are in complex and not direct interactors. Finally, HDA-1 SUMOylation is indicated to regulate MEP-1 interaction with numerous factors (Figure 3D). If all these factors are in one complex, it is hard to imagine how a single SUMO residue would mediate all of these simultaneously. It is quite likely (and not tested) that loss of HDA-1 SUMOylation leads to (partial?) dissociation of a large complex, rather than loss of individual interactions with the SUMO residue of HDA-1. Unlike claimed by the authors, there is no evidence that the "activity" of HDA-1 is regulated by SUMO modification.

2. Based on loss of MEP-1/HDA-1 interaction upon pie-1 RNAi and smo-1 RNAi (Figure 4B), the authors conclude that "SUMOylation of PIE-1 promotes the interaction of HDA-1 with MEP-1 in the adult germline".

The evidence that it is PEI-1 SUMOylation that is affecting MEP-1/HDA-1 interaction is fairly weak. In fact, based on Figure 4A, MEP-1 and HDA-1 interact without expression of PIE-1, and in PIE-1 K68R (sumoylation-deficient), although due to poor labeling of the panel it is not clear whether lane 1 and 4 refer to the WT pie-1 locus without tag or lack of pie-1.

In 4B the HDA-1 band that is present in L4440 but not in pie-1 or smo-1 RNAi is very faint, and in our experience such weak signal is not linear i.e., bands can disappear or appear depending on the exposure. Importantly, according to the data, seemingly unmodified HDA-1 immunoprecipitated with MEP-1 (Figure 4B). This data contradicts the authors' claim that "These findings suggest that in the adult germline only a small fraction of the HDA-1 protein pool, likely only those molecules that are SUMOylated, can be recruited by MEP-1 for the assembly of a functional NURD complex".

Furthermore, the fact that pie-1 and smo-1 depletion eliminate the interaction between HDA-1/MEP1 doesn't mean that the SUMOylation of pie-1 specifically is required for the interaction: perhaps un-SUMOylated pie1, and SUMOylation of something else, are both necessary for the interaction. The authors show that MEP-1 is also SUMOylated (Figure 3C). When IP-ing GFP-MEP-1, they precipitate all its modified forms and associated factors. One alternative possibility for why smo-1 RNAi abolishes MEP-1/HDA-1 interaction is that MEP-1 SUMOylation is needed for interaction with HDA-1 (independently of pie-1). (On a side note, why are the authors not including MEP-1 SUMOylation in the model?)

3. On page 13 the authors write: "These findings suggest that SUMOylation of PIE-1 on K68 enhances its ability to activate HDA-1 in the adult germline" and "We have shown that PIE-1 is also expressed in the adult germline where it engages the Krüppel-type zinc finger protein MEP-1 and the SUMO-conjugating machinery and functions to promote the SUMOylation and activation of the type 1 HDAC, HDA-1 (Figure 6)". Activation of HDA-1 is misleading and was never tested. If not performing in vitro assays for HDAC activity, the authors at least need to look at whether pie loss (degron) leads to acetylation of genomic HDA-1 targets and whether it affects HDA-1 (and/or MEP-1) recruitment to these sites. This could be done by ChIP-seq of HDA-1 and H3K9ac in WT and pie-1 degron animals.

https://doi.org/10.7554/eLife.63300.sa1

Author response

Essential revisions:

1. How sumoylation of K68 affects PIE-1 function, the nature of the SUMO E3 ligase that sumoylates PIE-1, whether sumoylated PIE-1 interacts directly with HDA-1, and, and if so, whether this requires interaction of the K68 SUMO moiety with HDA-1 (e.g. via a SIM) were not elucidated, and need to be addressed with new experimental data. For instance, does a SUMO::K68R PIE-1 fusion complement the pie-1 mutant, or is the exact site of PIE-1 sumoylation important? Also, in vitro deacetylase assays of the sort suggested in the decision letter for eLife-63299, are needed to determine if PIE-1 K68 sumoylation leads to increased HDA-1 enzymatic activity by comparing WT and K68R PIE-1 strains. Additional suggestions for investigating the interaction of PIE-1 with HDA-1 and UBC-9 can be found in Reviewer 1's point 1.

These comments made clear to us that we had placed too much emphasis on the downstream biochemical implications of our findings. We did not mean to imply that SUMO modification of HDAC increases its enzymatic activity; this possibility had not even occurred to us and seems very unlikely. The key value of our study is in the genetic insights it provides into the role of SUMO as a factor that along with PIE-1 promotes germline cell fates in the embryo and Argonaute-mediated surveillance and the assembly of an adult germline NuRD complex. We have extensively revised the paper to clarify these strengths of our story, and to remove confusion. Each of the above critiques are addressed throughout the paper, both with new experiments and with discussion.

We changed the title to downplay HDAC as the focus.

The last sentence of the Abstract now emphasizes our genetic findings and reads: “Our analysis of genetic interactions between pie-1 and sumo-pathway factors suggest that PIE-1 engages the SUMO machinery both to preserve the germline fate in the embryo and to promote Argonaute-mediated surveillance in the adult germline.”

Related to this last point: We now include a new section to the results examining synthetic genetic interactions between pie-1(K68R) and the SUMO E3 ligase homolog gei-17. These experiments show that while neither single mutant causes robust de-silencing, the double shows rapid and complete desilencing of the reporter. These experiments were difficult because they uncovered a haploinsufficiency. The new Results section relating this reads as follows:

“PIE-1 and GEI-17 act together to promote Piwi Argonaute-mediated silencing

In a parallel study exploring the role of SUMO and NuRD complex co-factors in piRNA-mediated silencing in the germline, we found that mutations in smo-1 and ubc-9 activate germline expression of a piRNA pathway reporter (Kim et al., parallel), but null alleles of gei-17 do not (Figure 6B). […] Thus PIE-1 and GEI-17 appear to function redundantly to promote piRNA surveillance and fertility in the adult germline.”

These new findings further support our new discussion of PIE-1 as an E3-like factor that acts in parallel with GEI-17.

How sumoylation of K68 affects PIE-1 function, the nature of the SUMO E3 ligase that sumoylates PIE-1.

The new Discussion also addresses these essential issues, and the new genetic data strongly support the idea that PIE-1 functions like an E3. It should also be emphasized that our findings clearly indicate how K68 affects PIE-1 activity from a genetic perspective. This is an important point, and it is not clear to us how additional mechanistic details would change the paramount importance of the key genetic findings. Unfortunately, this protein is not soluble, and without some kind of breakthrough, we don’t see how we could possibly address how K68 affects PIE-1 binding to other proteins.

Whether sumoylated PIE-1 interacts directly with HDA-1, and, and if so, whether this requires interaction of the K68 SUMO moiety with HDA-1 (e.g. via a SIM) were not elucidated, and need to be addressed with new experimental data.

Although we cannot address these questions due to the aforementioned solubility issues, we now include more data from our 2-hybrid studies. These 2-hybrid findings are discussed as they relate to the mechanism of HDA-1 regulation by PIE-1 and SUMO in the new Discussion section below:

“Because PIE-1 appears to interact directly with UBC-9, it is possible that PIE-1 harnesses the SUMO-conjugating machinery by acting like an E3 SUMO ligase both for itself and for target proteins. […] Thus PIE-1 may bind UBC-9 and MEP-1 simultaneously. Perhaps this ternary complex transiently associates with HDA-1 to promote its SUMOylation. HDA-1-SUMO might then associate with one or both of the putative SUMO-interacting motifs on MEP-1 (Kim et al., parallel).”

2. Additional supporting data, including in vitro experiments (and better controlled immunoblot exposures) are needed to prove that PIE-1 sumoylation is important for interactions between HDA-1 and PIE-1, UBC-9 and MEP-1. The current data are not convincing.

We apologize for the poor quality of some of our blots and the labeling that made it difficult to follow the subtle changes.

We do not provide any evidence that SUMOylation of PIE-1 alters direct physical interactions between PIE-1 and other factors. Again, the insolubility of PIE-1 prevents us from doing so. Instead we used the 2-hybrid, as discussed above, to find candidate interactors. To validate the interactions with UBC-9 and SUMO, it was necessary to undertake our proteomic studies of SUMO-binding proteins, which fortunately were possible under denaturing conditions. We feel that the worm SUMO proteome identified here is of extremely high quality and represents extensive efforts on the part of our collaborators in the laboratory of Dr. Men-Qiu Dong. This information and our reagents should be of significant value to the worm community.

In addition, we believe that the identification of PIE-1 as a SUMOylated protein and lysine 68 as a residue required for PIE-1 SUMOylation provide the kind of rigorous biochemical footing for our otherwise primarily in vivo genetic study. We show that pie-1 (genetic activity) promotes the SUMOylation of HDA-1 and also promotes the association of HDA-1 with MEP-1 and other components of the NuRD complex. We agree with the reviewers that the western blots that show this relatively weak association are underwhelming. This is why we undertook a whole parallel study to more directly explore the consequences of SUMO modifications on HDA-1.

We have carefully revised the results describing the PIE-1-dependence of HDA-1 SUMOylation to be more circumspect. We have relabeled the blots and repeated with fresh antibody that now more clearly show that HDA-1 is indeed SUMOylated, and that the levels are reduced in PIE-1(K68R) and in pie-1 and smo-1RNAi.

Additional points are raised in the individual reviews and could be addressed, if the authors believe that addressing them would strengthen the manuscript.

Reviewer #1:

The evidence that sumoylation of K68 in the PIE-1 zinc finger protein is important for HDA-1 type 1 histone deacetylase association and sumoylation seems reasonable, and, is important because as shown in the co-submitted paper HDA-1 sumoylation leads to its association with MEP-1 and LET-418/NuRD complex thus accelerating H3K9ac deacetylation, and silencing gene expression..

The evidence that PIE-1 is needed for sumoylation of HDA-1, presumably though association of PIE-1 with the UBC-9 SUMO E2, is reasonable. However, several aspects of the authors' model remain unclear, and there is an absence of biochemical assays to establish the role of sumoylated PIE-1 in HDA-1 sumoylation, and the effects of sumoylation on HDA-1 HDAC activity.

1. How sumoylation of K68 in PIE1 affects its function was not worked out. Can the deleterious effect of the K68R mutation on PIE-1 function be reversed by generating a SUMO-PIE-1 fusion, as was done for HDA-1 in the co-submitted paper? K68 maps to the N-terminal side of ZF1 in the PIE-1 protein in what appears to be an unstructured region.

Again, we have tried to emphasize in the revised papers that we have addressed the function of PIE-1 SUMOylation primarily with genetic studies, a strength of our system. Indeed, all of the alleles used in this study were generated at the endogenous loci by CRISPR HDR. The reviewer makes a good suggestion to attempt rescue of PIE-1(K68R) by appending SUMO through translational fusion. We attempted this with N-terminal, C-terminal, and internal fusions of SUMO into the endogenous pie-1orf. Unfortunately, all of these alleles caused complete embryonic lethality or strong sterility.

Does the SUMO residue play a role in the interaction of PIE-1 with HDA-1?

Again, because PIE-1 is insoluble, we cannot examine whether or not PIE-1 directly interacts with HDA-1. We show that PIE-1 and SUMO promote the interaction between HDA-1 and MEP-1, enabling them to form an adult-stage NuRD complex. K68R caused a reduction in the association between HDA-1 and MEP-1. PIE-1 does interact directly with MEP-1 and with SUMO machinery (based on 2-hybrid data).

Are the zinc fingers required for PIE-1 interaction with HDA-1 or UBC-9? No zinc finger mutations were tested.

We now include more discussion of PIE-1 two-hybrid interactions, as mentioned above, and describe how the region including the zinc fingers is required for the UBC-9 interaction, while the C-terminal proline-rich region is required for MEP-1 interactions. Mutations that alter or remove the zinc fingers of PIE-1 are not viable, making it difficult to assess their effect on the role of PIE-1 in promoting HDA-1 SUMOylation.

Does HDA-1 have a SIM that would allow it to interact selectively with sumoylated PIE-1?

There is no known SIM in HDAC. The prediction algorithm GPS-SUMO (Zhao et al., 2014) identifies one possible “low confidence” SIM in HDA-1. We have not had time to experimentally validate this one. However, as noted above we now discuss how, by forming a ternary complex with UBC-9 and MEP-1 (both of which interact strongly with PIE-1 in the 2-hybrid), PIE-1 may be able to engage and SUMOylate HDA-1 to promote its interaction with MEP-1 which does have SIM domains predicted with “high confidence” by GPS-SUMO.

Another, possibility is that the PIE-1 SUMO moiety is important because it interacts with the non-covalent SUMO-binding site on the backside of UBC-9 (Capill and Lima, JMB 369:606, 2007), which might stabilize the interaction. The backside interaction of SUMO with UBC-9 is proposed to promote UBC-9-mediated sumoylation of target proteins with SUMO consensus sites that are directly recognized by UBC-9. In this scenario, SUMO-PIE-1 would in effect be acting as an E3 SUMO ligase for HDA-1 by serving as a recruitment "factor". In this regard, the authors could test biochemically whether recombinant PIE-1 or K68SUMO-PIE-1 stimulates sumoylation of HDA-1 by UBC-9, using recombinant WT and KKRR mutant HDA-1 as substrates. These issues deserve discussion.

Thanks for these suggestions. As noted above we now discuss these ideas.

2. What is the SUMO E3 ligase that sumoylates PIE-1? Is it possible that through association with UBC-9, perhaps through its zinc fingers, PIE-1 is sumoylated in cis within a PIE-1/UBC-9 complex?

As noted above, we now discuss this important issue of E3 activities in considerable detail.

3. In many places, including the title, the authors make the claim that PIE-1 promotes sumoylation and activation of HDA-1. While it is clear that PIE-1 does increase sumoylation of HDA-1, in a manner requiring K68, and that H3K9ac levels are decreased as a result, the authors do not provide any direct evidence that this process increases HDA-1 catalytic activity, as is implied in the title and elsewhere. As indicated in the review of the co-submitted paper, this would need to be established by carrying out an HDAC assay on control and sumoylated HDA-1 in vitro. Instead of enzymatic activation, it is possible that the PIE-1 interaction and HDA-1 sumoylation results in relocalization of HDA-1 within the nucleus to facilitate more efficient H3K9ac deacetylation.

Again, we apologize for this confusion. We never meant to imply that the enzymatic activity of HDA-1 is increased by SUMOylation. We have carefully removed this wording throughout the manuscript. We think it is far more likely that HDA-1 SUMOylation promotes hypoacetylation of H3K9 by promoting the association of HDA-1 with its adult germline NuRD co-factors (as alluded to in the last comment from the reviewer above). We would be very surprised to find that a purified HDA-1::SUMO protein by itself has greater enzymatic activity. If that were to prove true, it would no doubt require a great deal of further investigation in order to provide meaningful understanding at a structural and biochemical level. Such studies and in vitro assays would go well beyond the primarily genetic and molecular studies of the kind presented here.

Reviewer #2:

In their manuscript, Kim et al. address the role of PIE-1 sumoylation during C. elegans oogenesis. The authors favour a model in which sumoylated PIE-1 acts as a sort of E3-like factor 'enhancing' HDA-1 sumoylation. While the results are indeed very interesting, it is unclear to me whether there is enough data to support the author's model. I have list of comments, suggestions, questions, and concerns, which are listed below, which I hope will help the authors strengthen the manuscript:

Figure 1:

i. As with the accompanying manuscript, the extremely low level of SUMO modification should be factored in the model.

Thank you. As noted above we have added a discussion of this important issue.

ii. Is sumoylation also observed in untagged pie-1? As juged by figure 3A, the authors have a very good antibody to test this.

Unfortunately, the antibody is a monoclonal that, by chance, was raised against the peptide that includes K68. In all of our tests this antibody fails to detect the SUMOylated isoform of the protein.

iii. While the authors claim that PIE-1 sumoylation is not observed in embryos, that panel show a lower exposure than the corresponding one in Adult (as judged by the co-purified unmodified PIE-1::FLAG). A longer exposure and/or more loading would be helpful.

We have repeated this experiment and now include a longer exposure and arrows to indicate the expected size of the PIE-1-SUMO band. There is a background band that runs slightly higher in the blot, but we think the loadings are now comparable and clearly show that PIE-1 is modified by SUMO in adults but not detectably in embryos.

iv. Their strategy and optimisation for purification of sumoylated proteins is excellent and will be useful for future research (along with other reagents the authors developed here).

We thank the reviewer for these kind words. Our collaborators have developed state of the art Mass Spec data on the worm SUMO proteome.

Is the 10xHis::smo-1 functional? Could this be tested in vitro and/or in vivo?

Yes. As we now state clearly in the paper, the HIS tag is inserted at the endogenous smo-1 locus (the only worm SUMO gene), and the strain is fully viable and healthy. This is very important as noted above, as it enables experiments like ours that identify critical lysines in the targets so that specific genetic tests of the importance of SUMO modifications on each substrate can be analyzed.

v. In vitro PIE-1 sumoylation would be a desirable addition to this figure.

We provide in vivo genetic evidence that PIE-1 and SUMO function together in both the embryo and the adult. We have directly identified PIE-1 SUMOylation in vivo with sensitive Ni-affinity and western blot studies on worm lysates, using tags engineered at the endogenous smo-1 and pie-1 alleles. We have also shown quite clearly – again with direct in vivo studies – that K68 is required for SUMOylation of PIE-1. We say more on this below in response to your concluding statement.

vi. In addition to germline PIE-1 localisation, it would be interesting to see embryos and PIE-1(K68R).

We now include these images as a Supplementary figure (Figure 1—figure supplement 3).

vii. MW markers are missing in the blots.

We have added markers to indicate the MW in each blot.

Figure 2:

i. The generation of the ubc-9 ts allele is an exceptional tool. Could the authors show SUMO conjugation levels at permissive vs restrictive temperature? Just out of curiosity, is this a fast-acting allele?

Thanks. Yes, this is a fast-acting and reversible ts allele, so we hope it will prove useful to the community. We are glad to make it available, although it is also very easy to CRISPR it in. Based on our genetic tests the protein is a weak hypomorph (slightly reduced function), but we have not tested its SUMO-conjugating activity by comparing substrates at the permissive and non-permissive temperature.

ii. The authors mention that gei-17 alleles are viable, could the authors mention any thoughts on why the tm2723 allele is lethal/sterile?

In our hands gei-17 null alleles are homozygous viable, but produce a mixture of ~70% sterile adults and ~2% dead embryos in each brood. We have not analyzed tm2723, but note that it is available as an unbalanced (homozygous) strain according to wormbase.

Figure 3:

i. Panel C is mentioned in the text in the wrong place. Also in C, what do the authors think about the big increase in MEP-1 sumoylation in the PIE-1(K68R) background?

We have corrected the figure calls, and we have rearranged the figure to more clearly and concisely indicate the embryo and adult studies. You are right, MEP-1 SUMOylation does seem to be increased slightly in the mutant and in pie-1(RNAi). However, we have not identified the SUMO acceptor lysines nor generated any functional data indicating the importance (if any) of MEP-1 SUMOylation. Investigating this modification to MEP-1 will require a future study.

ii. I have the same comment for panel D as I had for figure 1 comment III: the exposure/loading for the embryo WB seems lower, as judged by the co-purifying, unmodified HDA-1. A positive control for sumoylated protein coming from embryos would be nice.

We have adjusted the loading and include MEP-1 as a positive control for a SUMOylated protein from embryos.

iii. In general, the model of PIE-1 acting as a SUMO machinery recruiter should be tested with recombinant proteins. Even if compatible with some results in vivo, showing that this is a plausible mechanism in vitro would be extremely helpful and greatly support the authors' claim.

We thank the reviewer for this perspective. We agree that in vitro studies would be helpful in the future, especially if they help uncover factors or modifications that cause adult germline and embryo MEP-1 Mi2/LET-418 complexes to differ so dramatically in their association with HDA-1. Especially if these factors—whatever they are—turn out to be highly conserved proteins (unlike PIE-1). Until that problem is solved, even if PIE-1 could be shown to promote HDA-1 SUMOylation in vitro with purified components, it would be unlikely to modulate the association of HDA-1 with MEP-1 in vitro, as the aforementioned modifications or co-factors that suppress/promote their association are not yet in hand.

At present, our genetic arguments strongly support the idea that PIE-1 works together with SUMO components to carry out its functions. We feel like our hard fought gains in understanding and revealing a potential mechanism for PIE-1 adult germline function (by promoting HDAC NuRD complex assembly) are very significant given the strong context of the entirely in vivo genetic backdrop for these whole animal studies. We feel like this genetic in vivo aspect of the story is solid and very interesting and is already well-supported by good molecular genetic studies using endogenous alleles throughout.

Figure 4:

i. The authors make a quantitative comparison of the HDA-1/MEP-1 interaction in the text. I think this is not correct. Even if these have been run in the same gel, this could just be a lower exposure. In this line, the HDA-1 blot in the 'Adult' IP would benefit from a longer exposure to better appreciate what seems a rather small difference between PIE-1 and PIE-1(K68R).

We now include a longer exposure that helps to make this difference more clear. It should be noted that the SUMO-dependence of this interaction is pursued more directly and completely in our parallel story on HDAC SUMOylation. Although it may seem weak, it is most definitely real and, we believe, important. In the revised Discussion, we suggest that this apparently weak association is likely misleading due to SUMO reversal during IP incubations.

ii. Since there still seems to be interaction between MEP-1 and HDA-1 in the PIE-1(K68R) background, does smo-1(RNAi) or ubc-9(G56R) reduce this further?

As indicated in the revised Figure 4, lanes 31 and 32, both pie-1(RNAi) and smo-1(RNAi) appear to reduce this interaction further.

iii. In panel B, the LET-418 blot on the right is massively overexposed.

We provide a shorter exposure, but LET-418 interacts very robustly with MEP-1 in adult lysates, which is what we were trying to illustrate. When relative exposures are adjusted to detect HDA-1, this over-exposure happens to the LET-418 western.

iv. Once again, in vitro binding experiments to get some indication that the authors' model is plausible would be a great addition.

Thanks again for this comment. We have responded to this issue of in vitro studies above. But please clarify if there are specific new in vitro experiments you have in mind. Again, the genetic arguments we make are very well supported by molecular genetic studies and by yeast two-hybrid data.

It is not clear what aspect of our model seems implausible. We do agree with the reviewer that the role of PIE-1 in promoting HDA-1 SUMOylation and its role in the regulation of the adult stage MEP-1–HDA-1 interaction remains somewhat tentative (but is addressed more deeply in the second paper). But we don’t think they are implausible. In the revised manuscript, we have de-emphasized these molecular details (taking them out of the title, for example). We think the findings that PIE-1 is SUMOylated and acts through SUMO to regulate gene expression in both the adult and embryo germlines are important and well-established aspects of our paper. As noted above, the importance of HDAC SUMOylation is addressed much more completely in the parallel submission.

Figure 5:

i. Could the authors make some quantitation of the immunofluorescence data?

We now include quantification (Figure 5B).

Overall, I think this manuscript proposes a very interesting model and the results support this model, although I am not convinced these are sufficient to strongly back the authors' claims. I would very much like to see a revised version with some in vitro data backing the authors' model.

We hope the reviewer will be satisfied with the revisions we have made to emphasize the molecular genetic (rather than biochemical) focus of our work. We have emphasized and expanded on our 2-hybrid data in order to help address this need for in vitro mechanistic binding information. PIE-1 is a difficult protein in terms of solubility, both in vivo and in our limited attempts to work with it in vitro. It is also a novel protein, that beyond its tandem zinc fingers is not conserved. So detailed in vitro insights into how PIE-1 SUMOylation changes its function are unlikely to be of great interest to the readers of eLife. As noted earlier, a key mystery that deserves further investigation at the biochemical level is why HDA-1 fails to associate with the NuRD complex in the adult germline, in the first place. In any event, thanks for your careful consideration of our work, and we apologize that we cannot be more forthcoming with in vitro data.

Reviewer #3:

In the manuscript by Kim et al., show that, beyond its roles of preventing somatic differentiation in the germline of embryos, Zn-finger protein PIE-1 also functions in the adult germline, where it is both SUMOylated as well as interacts with the SUMO conjugating machinery and promotes SUMOylation of protein targets. They identify HDA-1 as a target of PIE-1-induced SUMOylation. Here too, I find the claims interesting, however data is sometimes missing or does not fully support the claims.

1. A key claim of novelty over previously proposed "glue" functions of SUMO is based on the fact that they find that temporally regulated SUMOylation of a very specific residue in a specific protein is affecting protein activity: The observation that "SUMOylation of HDA-1 only appears to regulate its functions in the adult germline" and not in the embryo together with the finding that "other co-factors such as MEP-1 are SUMOylated more broadly, these findings imply that SUMOylation in the context of these chromatin remodeling complexes, does not merely function as a SUMO-glue (Matunis et al., 2006) but rather has specificity depending on which components of the complex are modified and/or when."

I find this claim poorly supported by the data. In fact, I find that the data supports that multiple SUMOylations contribute to formation of larger complexes: The His-SUMO IP (Figure 2B) brings down far more un-SUMOylated HDA-1 than SUMOylated. This argues for the presence of large complexes with different factors being SUMOylated and many bringing down unmodified HDA-1.

As we stated in the paper, the Ni-affinity enrichments are performed under denaturing conditions and therefore do not pull down complexes bridged by protein-protein interactions. This is why PIE-1 protein which is otherwise not soluble, was recovered using this method. The non-SUMOylated proteins recovered in these experiments are brought down individually (not in complexes), and presumably this is due to unavoidable background binding between the Ni resin and clusters of Histidines in these proteins. Background binding to the resin is different for every protein, and is not by itself a useful measure of the relative SUMOylation level of the protein. We now explain the procedure and emphasize the points more strongly in the revised paper. Thanks for pointing out these issues as no doubt many other readers would be unfamiliar with such details.

The chromatography experiments (Figure 3B-C) also provide hits that are in complex and not direct interactors.

The reviewer is referring to Figure 3 in the HDA-1 paper, not this paper. Again, the histograms compare the recovery of proteins by Ni-affinity chromatography under denaturing conditions, which does not capture protein complexes. We have clarified in both papers that Ni-affinity chromatography was done under denaturing conditions, and we apologize for the confusion.

Finally, HDA-1 SUMOylation is indicated to regulate MEP-1 interaction with numerous factors (Figure 3D). If all these factors are in one complex, it is hard to imagine how a single SUMO residue would mediate all of these simultaneously.

Yes, we agree; this is a striking finding. Appending SUMO by translational fusion to HDA-1 results in a dramatic increase in the co-IP between MEP-1, HDA-1, and several other factors that are known to form complexes with HDA-1. As we discuss in the paper, appending SUMO to HDA-1 seems to overcome a barrier to its interaction with MEP-1 and enables the proteins to assemble a functional NuRD complex in the adult germline.

It is quite likely (and not tested) that loss of HDA-1 SUMOylation leads to (partial?) dissociation of a large complex, rather than loss of individual interactions with the SUMO residue of HDA-1.

We don’t understand this comment, which again seems to be addressing the HDA-1 paper, not this paper. Perhaps the reviewer did not understand that we pulled down MEP-1 not HDA-1 in Figure 3D of the HDA-1 paper.

Unlike claimed by the authors, there is no evidence that the "activity" of HDA-1 is regulated by SUMO modification.

We apologize again for this misunderstanding. We agree that SUMO is unlikely to alter the HDA-1 enzymatic activity. Rather as now more clearly stated throughout the paper, we believe it alters its activity toward its histone substrates by enhancing its association with MEP-1.

2. Based on loss of MEP-1/HDA-1 interaction upon pie-1 RNAi and smo-1 RNAi (Figure 4B), the authors conclude that "SUMOylation of PIE-1 promotes the interaction of HDA-1 with MEP-1 in the adult germline".

The evidence that it is PEI-1 SUMOylation that is affecting MEP-1/HDA-1 interaction is fairly weak. In fact, based on Figure 4A, MEP-1 and HDA-1 interact without expression of PIE-1, and in PIE-1 K68R (sumoylation-deficient), although due to poor labeling of the panel it is not clear whether lane 1 and 4 refer to the WT pie-1 locus without tag or lack of pie-1.

Again we apologize for the confusion and poor labeling of our figures. We now make it clear that all of the strains are wildtype for PIE-1 function with the exception of those expressing PIE-1(K68R) or exposed to pie-1(RNAi). The dash was meant to indicate the absence of the tag not the protein or gene activity. In the original figure, the top panels showed results from adult lysates, and the bottom panels showed results from embryo lysates. As we note in the paper and as mentioned by the reviewer, HDA-1 and MEP-1 interact robustly in embryos regardless of the SUMOylation status of HDA-1. To make the experiments and results clearer, we now place the two conditions—Adult and Embryo—side by side and color code them. We also put the most important blots (HDA-1) on top and call out all the key lanes by number. As noted above and now emphasized throughout the paper, the interaction between MEP-1 and HDA-1 is weak in the Adult stage, and this weak interaction requires PIE-1 activity and is promoted by PIE-1 SUMOylation. We also now make a point of discussing how this apparently weak interaction may be a detection problem due to reversal of SUMO in the IP lysates.

In 4B the HDA-1 band that is present in L4440 but not in pie-1 or smo-1 RNAi is very faint, and in our experience such weak signal is not linear i.e., bands can disappear or appear depending on the exposure.

Under the conditions used in our study, a relatively very small amount of HDA-1 is recovered in the MEP-1 IPs from the adult germline compared to the embryo. We also include longer exposures now that show this better. The interaction is reproducible, and is consistently reduced in K68R, pie-1(RNAi), and smo-1(RNAi) worms. In contrast Mi2/LET-418 interacts robustly with MEP-1 at all stages and in all genetic contexts. We intentionally exposed the blots from Adults and Embryos for equal amounts of time so that the relative amount of LET-418 blot and HDA-1 recovered in the IPs could be compared directly. Hence the over-exposure of LET-418 and under-exposure of the HDA-1. At the request of the reviewers, we have added additional figures showing longer exposures of HDA-1 in the Adult stage coIP.

Importantly, according to the data, seemingly unmodified HDA-1 immunoprecipitated with MEP-1 (Figure 4B). This data contradicts the authors' claim that "These findings suggest that in the adult germline only a small fraction of the HDA-1 protein pool, likely only those molecules that are SUMOylated, can be recruited by MEP-1 for the assembly of a functional NURD complex".

We thank the reviewer for pointing this out, and again we apologize for not explaining this finding better. SUMO modifications are transient and reversible and are often subject to reversal by de-SUMOylating machinery during incubation in IP lysates. We now address this issue directly in the Results and Discussion sections and include a figure (1D) to illustrate this rapid de-conjugation of SUMO from substrates in IP buffer.

Furthermore, the fact that pie-1 and smo-1 depletion eliminate the interaction between HDA-1/MEP1 doesn't mean that the SUMOylation of pie-1 specifically is required for the interaction: perhaps un-SUMOylated pie1, and SUMOylation of something else, are both necessary for the interaction.

We agree with the reviewer. We show that PIE-1(K68R) reduces but does not eliminate the interaction, and we speculate that PIE-1, even when not SUMOylated can promote the interaction. Our best evidence is genetic, so of course it could be indirect. However, PIE-1 does directly interact with MEP-1, and with SUMO and UBC-9, so a direct modification of HDA-1 is certainly plausible. We have better explained and de-emphasized this detail and hope this makes the paper more acceptable to the reviewer.

The authors show that MEP-1 is also SUMOylated (Figure 3C). When IP-ing GFP-MEP-1, they precipitate all its modified forms and associated factors. One alternative possibility for why smo-1 RNAi abolishes MEP-1/HDA-1 interaction is that MEP-1 SUMOylation is needed for interaction with HDA-1 (independently of pie-1). (On a side note, why are the authors not including MEP-1 SUMOylation in the model?)

MEP-1 is SUMOylated in both the embryo and the adult, as are additional components of the NuRD complex. While it’s possible that this modification is essential for its (their) functions in one or both tissues, we have not explored this yet. A careful exploration of this question will require finding and mutating the acceptor lysines.

3. On page 13 the authors write: "These findings suggest that SUMOylation of PIE-1 on K68 enhances its ability to activate HDA-1 in the adult germline" and "We have shown that PIE-1 is also expressed in the adult germline where it engages the Krüppel-type zinc finger protein MEP-1 and the SUMO-conjugating machinery and functions to promote the SUMOylation and activation of the type 1 HDAC, HDA-1 (Figure 6)". Activation of HDA-1 is misleading and was never tested.

We did not mean to imply enzymatic activity was increased. This section has been totally revised to stress the key genetic findings.

If not performing in vitro assays for HDAC activity, the authors at least need to look at whether pie loss (degron) leads to acetylation of genomic HDA-1 targets and whether it affects HDA-1 (and/or MEP-1) recruitment to these sites. This could be done by ChIP-seq of HDA-1 and H3K9ac in WT and pie-1 degron animals.

Thanks for the suggestion, it is difficult/impossible to collect enough material by dissecting gonads to be able to perform ChIP seq studies on adult germline tissue from worms. One solution is to drive a tagged transgene and perform ChIP that way. We did this in the HDA-1 paper. However, we felt that performing mRNA seq on the actual mutant alleles, directly, gives a similar read out on overlap between targets. We now include direct comparisons of up-regulated genes in dissected gonads from hda-1([KKRR]), mep-1::degron, and pie-1::degron, showing strong overlaps (Figure 5F).

https://doi.org/10.7554/eLife.63300.sa2

Article and author information

Author details

  1. Heesun Kim

    RNA Therapeutics Institute, University of Massachusetts Medical School, Worcester, United States
    Contribution
    Conceptualization, Data curation, Formal analysis, Validation, Investigation, Visualization, Methodology, Writing - original draft, Writing - review and editing
    Contributed equally with
    Yue-He Ding
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0001-7643-4516

  2. Yue-He Ding

    RNA Therapeutics Institute, University of Massachusetts Medical School, Worcester, United States
    Contribution
    Data curation, Formal analysis, Validation, Investigation, Visualization, Writing - original draft, Writing - review and editing
    Contributed equally with
    Heesun Kim
    Competing interests
    No competing interests declared

  3. Shan Lu

    National Institute of Biological Sciences, Beijing, China
    Contribution
    Formal analysis, Investigation
    Competing interests
    No competing interests declared

  4. Mei-Qing Zuo

    National Institute of Biological Sciences, Beijing, China
    Contribution
    Investigation
    Competing interests
    No competing interests declared

  5. Wendy Tan

    RNA Therapeutics Institute, University of Massachusetts Medical School, Worcester, United States
    Contribution
    Validation, Investigation
    Competing interests
    No competing interests declared

  6. Darryl Conte Jr

    RNA Therapeutics Institute, University of Massachusetts Medical School, Worcester, United States
    Contribution
    Conceptualization, Writing - review and editing
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-1137-8901

  7. Meng-Qiu Dong

    National Institute of Biological Sciences, Beijing, China
    Contribution
    Supervision, Investigation
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0002-6094-1182

  8. Craig C Mello

    1. RNA Therapeutics Institute, University of Massachusetts Medical School, Worcester, United States
    2. Howard Hughes Medical Institute, Chevy Chase, United States
    Contribution
    Conceptualization, Supervision, Investigation, Writing - original draft, Writing - review and editing
    For correspondence
    Craig.Mello@umassmed.edu
    Competing interests
    No competing interests declared
    ORCID icon "This ORCID iD identifies the author of this article:" 0000-0001-9176-6551

Funding

Howard Hughes Medical Institute

  • Craig C Mello

NIH Office of the Director (GM58800)

  • Craig C Mello

The funders had no role in study design, data collection and interpretation, or the decision to submit the work for publication.

Acknowledgements

We thank members of Mello and Ambros labs for discussions. CCM is a Howard Hughes Medical Institute Investigator.

Senior Editor

  1. Kevin Struhl, Harvard Medical School, United States

Reviewing Editor

  1. Tony Hunter, Salk Institute for Biological Studies, United States

Reviewers

  1. Tony Hunter, Salk Institute for Biological Studies, United States
  2. Federico Pelisch, University of Dundee, United Kingdom

Version history

  1. Received: September 21, 2020
  2. Accepted: April 23, 2021
  3. Version of Record published: May 18, 2021 (version 1)

Copyright

© 2021, Kim et al.

This article is distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use and redistribution provided that the original author and source are credited.

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  1. Heesun Kim
  2. Yue-He Ding
  3. Shan Lu
  4. Mei-Qing Zuo
  5. Wendy Tan
  6. Darryl Conte Jr
  7. Meng-Qiu Dong
  8. Craig C Mello
(2021)
PIE-1 SUMOylation promotes germline fates and piRNA-dependent silencing in C. elegans
eLife 10:e63300.
https://doi.org/10.7554/eLife.63300

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    Yoshifumi Sonobe, Soojin Lee ... Paschalis Kratsios
    Research Article Updated

    A hexanucleotide repeat expansion in C9ORF72 is the most common genetic cause of amyotrophic lateral sclerosis (ALS) and frontotemporal dementia (FTD). A hallmark of ALS/FTD pathology is the presence of dipeptide repeat (DPR) proteins, produced from both sense GGGGCC (poly-GA, poly-GP, poly-GR) and antisense CCCCGG (poly-PR, poly-PG, poly-PA) transcripts. Translation of sense DPRs, such as poly-GA and poly-GR, depends on non-canonical (non-AUG) initiation codons. Here, we provide evidence for canonical AUG-dependent translation of two antisense DPRs, poly-PR and poly-PG. A single AUG is required for synthesis of poly-PR, one of the most toxic DPRs. Unexpectedly, we found redundancy between three AUG codons necessary for poly-PG translation. Further, the eukaryotic translation initiation factor 2D (EIF2D), which was previously implicated in sense DPR synthesis, is not required for AUG-dependent poly-PR or poly-PG translation, suggesting that distinct translation initiation factors control DPR synthesis from sense and antisense transcripts. Our findings on DPR synthesis from the C9ORF72 locus may be broadly applicable to many other nucleotide repeat expansion disorders.

    1. Ecology
    2. Genetics and Genomics

    Adulis and the transshipment of baboons during classical antiquity

    Franziska Grathwol, Christian Roos ... Gisela H Kopp
    Research Advance

    Adulis, located on the Red Sea coast in present-day Eritrea, was a bustling trading centre between the first and seventh centuries CE. Several classical geographers--Agatharchides of Cnidus, Pliny the Elder, Strabo-noted the value of Adulis to Greco--Roman Egypt, particularly as an emporium for living animals, including baboons (Papio spp.). Though fragmentary, these accounts predict the Adulite origins of mummified baboons in Ptolemaic catacombs, while inviting questions on the geoprovenance of older (Late Period) baboons recovered from Gabbanat el-Qurud ('Valley of the Monkeys'), Egypt. Dated to ca. 800-540 BCE, these animals could extend the antiquity of Egyptian-Adulite trade by as much as five centuries. Previously, Dominy et al. (2020) used stable istope analysis to show that two New Kingdom specimens of P. hamadryas originate from the Horn of Africa. Here, we report the complete mitochondrial genomes from a mummified baboon from Gabbanat el-Qurud and 14 museum specimens with known provenance together with published georeferenced mitochondrial sequence data. Phylogenetic assignment connects the mummified baboon to modern populations of Papio hamadryas in Eritrea, Ethiopia, and eastern Sudan. This result, assuming geographical stability of phylogenetic clades, corroborates Greco-Roman historiographies by pointing toward present-day Eritrea, and by extension Adulis, as a source of baboons for Late Period Egyptians. It also establishes geographic continuity with baboons from the fabled Land of Punt (Dominy et al., 2020), giving weight to speculation that Punt and Adulis were essentially the same trading centres separated by a thousand years of history.