Skip to main content
Download PDF

CDE-1 suppresses the production of risiRNA by coupling polyuridylation and degradation of rRNA

BMC Biology volume 18, Article number: 115 (2020) Cite this article

Abstract

Background

Modification of RNAs, particularly at the terminals, is critical for various essential cell processes; for example, uridylation is implicated in tumorigenesis, proliferation, stem cell maintenance, and immune defense against viruses and retrotransposons. Ribosomal RNAs can be regulated by antisense ribosomal siRNAs (risiRNAs), which downregulate pre-rRNAs through the nuclear RNAi pathway in Caenorhabditis elegans. However, the biogenesis and regulation of risiRNAs remain obscure. Previously, we showed that 26S rRNAs are uridylated at the 3′-ends by an unknown terminal polyuridylation polymerase before the rRNAs are degraded by a 3′ to 5′ exoribonuclease SUSI-1(ceDIS3L2).

Results

Here, we found that CDE-1, one of the three C.elegans polyuridylation polymerases (PUPs), is specifically involved in suppressing risiRNA production. CDE-1 localizes to perinuclear granules in the germline and uridylates Argonaute-associated 22G-RNAs, 26S, and 5.8S rRNAs at the 3′-ends. Immunoprecipitation followed by mass spectrometry (IP-MS) revealed that CDE-1 interacts with SUSI-1(ceDIS3L2). Consistent with these results, both CDE-1 and SUSI-1(ceDIS3L2) are required for the inheritance of RNAi.

Conclusions

This work identified a rRNA surveillance machinery of rRNAs that couples terminal polyuridylation and degradation.

Background

RNAs are extensively modified: 5′ termini are often capped, internal positions are altered on both ribose rings and bases, and 3′ termini receive untemplated nucleotides, which are referred to as tails. In eukaryotes, tails occur on most classes of RNAs, and they control RNA processing, stability, transport, and function. Terminal modification is critical in biology. For example, uridylation is implicated in tumorigenesis, proliferation, stem cell maintenance, and immune defense against viruses and retrotransposons [1,2,3,4,5,6]. The C. elegans genome encodes three polyuridylation polymerases (PUPs): cde-1/pup-1/cid-1, pup-2, and pup-3 [7]. These PUPs may have distinct roles in different cellular contexts. cde-1 is involved in the inheritance of RNAi, chromosome segregation, and antiviral defense [4, 8, 9]. CDE-1 functions with the RNA-dependent RNA polymerase (RdRP) EGO-1 and the Argonaute CSR-1 in the germline to affect chromosome segregation [10]. PUP-2/3 are the homologs of TUT4/7 (terminal uridylyl transferases 4/7) in mammals. PUP-2 targets the microRNA let-7 and regulates the stability of LIN-28 [11]. The balance of CDE-1, PUP-2, and PUP-3 activities appears to ensure proper germline development in C. elegans [12].

Ribosome biogenesis is a very sophisticated multistep process, in which mistakes can occur at any step. Cells must carefully surveil the steps of the pre-rRNA processing and the assembly of ribosomal subunits. Misprocessed rRNAs are usually surveyed and degraded by multiple supervision machineries, including the exosome complex and the Trf4/Air2/Mtr4p polyadenylation (TRAMP) complex [13,14,15]. Aberrant RNAs are degraded by exosomes in a 3′-5′ exonucleolytic decay manner [16,17,18]. The exosome-independent exoribonuclease DIS3L2 plays a pivotal role in the 3′-5′ degradation of oligouridylated RNA fragments [19,20,21,22,23].

In addition to guiding erroneous rRNA degradation, antisense ribosomal siRNAs (risiRNAs) silence pre-rRNAs through the nuclear RNAi pathway to suppress the accumulation of erroneous rRNAs in C. elegans [20, 24,25,26]. Erroneous rRNAs are usually oligouridylated at the 3′-ends and then degraded by the exoribonuclease SUSI-1(ceDis3L2). However, it is unclear which terminal uridyltransferase performs the untemplated addition of the 3′-end uracil. Identifying which PUP is involved in the 3′-uridylation of erroneous rRNAs and how it is involved will further our understanding of the quality control mechanism of cellular nucleic acids.

Here, we found that CDE-1 is specifically involved in suppressing risiRNA production. CDE-1 localizes to perinuclear granules in the germline and uridylates both Argonaute-associated 22G-RNAs, 26S, and 5.8S rRNAs at the 3′-ends. Interestingly, we found that CDE-1 interacts with SUSI-1(ceDIS3L2). Both CDE-1 and SUSI-1(ceDIS3L2) are required for the inheritance of RNAi. Therefore, our findings are consistent with the model that CDE-1 suppresses generation of risiRNAs by uridylating rRNA and recruiting SUSI-1(ceDIS3L2) to the rRNA.

Results

Depletion of CDE-1 promotes risiRNA production

There are three RNA terminal uridylyltransferase genes, cde-1, pup-2, and pup-3, which are involved in RNA 3′-end uridylation in C. elegans. We previously showed that risiRNA was enriched in WAGO-4-bound siRNAs in cde-1 mutants [8]. To further study the specificity and function of cde-1 in risiRNA production, we used the GFP::NRDE-3 transgene as a reporter. NRDE-3 is an Argonaute protein that transports siRNAs from the cytoplasm to the nucleus [27]. NRDE-3 localizes to the nucleus when it binds to siRNAs, but it accumulates in the cytoplasm when not bound to siRNA ligands. Disruption of the generation of endogenous siRNAs, for example, loss of function of eri-1 mutant results in relocalization of NRDE-3 from the nucleus to the cytoplasm. We crossed eri-1(mg366);GFP::NRDE-3 onto the pup mutant lines and found that the depletion of cde-1, but not pup-2 or pup-3, was able to redistribute NRDE-3 from the cytoplasm to the nucleus (Fig. 1a). We generated a single copy transgene CDE-1::mCherry by Mos1-mediated single-copy insertion (MosSCI) technology. This transgene was able to rescue the cde-1(tm936) defects and redistribute NRDE-3 from the nucleus to the cytoplasm (Additional file 1: Fig. S1 A). To exclude the possibility that PUP-2 and PUP-3 act redundantly to suppress siRNA generation, we generated pup-2;pup-3 double mutants. In the double mutants, NRDE-3 still accumulated in the cytoplasm (Additional file 1: Fig. S1 B). These data suggest that NRDE-3 was bound to newly generated siRNAs in cde-1 mutants.

Fig. 1
figure 1

Antisense ribosomal siRNA (risiRNA) accumulats in cde-1 mutant. a NRDE-3 localized to the nucleus in eri-1(mg366);cde-1(tm936);GFP::NRDE-3 animals. Images show representative seam cells of the indicated animals. The percentage of animals with nuclear-enriched NRDE-3 in seam cells is indicated (% N). The number of scored animals is indicated in parentheses. White arrows, nucleus. b The risiRNA sensor was silenced in the cde-1 mutant. (Top) Schematic representation of the risiRNA sensor. (Middle) Images of C. elegans embryos with the indicated genotypes expressing the risiRNA sensor at the ~ 300-cell stage. The levels of GFP expression were scored for each genotype in the bottom panel. c qRT-PCR analysis of risiRNA levels in indicated animals at the L3 stage. Data are presented as the mean ± SD (n = 3, biological replicates). ns, not significant. **P < 0.01 (two-tailed Student’s t test). d, e Deep sequencing of NRDE-3-associated siRNAs in indicated animals. The red dashed line indicates risiRNAs. f The number of risiRNAs targeting the each region of pre-rRNA transcription unit were analyzed

Full size image

To test whether the NRDE-3-bound siRNAs in cde-1 mutants contain risiRNA sequences, we used a risiRNA sensor expressing a his-72p::gfp::his-72 reporter fused to the 26S rRNA sequence (Fig. 1b). The sensor was expressed in wild-type N2 and eri-1(mg366) animals but silenced in cde-1(tm936) mutants. Furthermore, we quantified the amount of risiRNA by quantitative real-time PCR analysis and found that risiRNAs were increased in cde-1 mutants, but not in pup-2 or pup-3 mutants (Fig. 1c).

Last, we immunoprecipitated NRDE-3 and deep sequenced its associated small RNAs in eri-1(mg366);GFP::NRDE-3 and eri-1(mg366);cde-1(tm936);GFP::NRDE-3 animals in a 5′-phosphate-independent manner. Notably, the proportion of NRDE-3-bound risiRNAs increased approximately 164-fold in eri-1(mg366);cde-1(tm936);GFP::NRDE-3 animals compared to the values observed in control animals (Fig. 1d, e). The abundance of risiRNAs targeting each rRNA region increased in cde-1(tm936) animals (Fig. 1f).

To search for the genetic requirements of risiRNA production in the cde-1 mutants, we crossed rrf-1, rrf-2, and rrf-3 lines onto the eri-1(mg366);cde-1(tm936);GFP::NRDE-3 animals. RRF-1, RRF-2, and RRF-3 are RNA-dependent RNA polymerases that are important for the generation of 22G-RNAs in C. elegans. Consistent with previous results, the depletion of rrf-1 and rrf-2 together resulted in NRDE-3 being redistributed from the nucleus to the cytoplasm (Additional file 1: Fig. S1 C). In addition, the depletion of rrf-1 and rrf-2 together partially restored the fecundity of eri-1;cde-1 animals (Additional file 1: Fig. S1 D).

Base on the above results, we conclude that cde-1 likely acts as a suppressor of siRNA (susi) gene and suppresses the generation of risiRNAs.

CDE-1 uridylates risiRNA

We first compared the small RNA expression profiles between wild-type and cde-1 mutant animals. Small RNAs were isolated from young adult animals. Although the depletion of cde-1 did not noticeably change the expression profile of different small RNA categories, risiRNAs were enriched 4.7 fold in cde-1 mutant animals vs wild-type animals (Fig. 2a). We then immunoprecipitated GFP::NRDE-3 and deep sequenced the associated siRNAs. NRDE-3-bound risiRNAs were enriched 17 fold in cde-1 mutant animals, compared to what was observed in control animals (Fig. 2b).

Fig. 2
figure 2

CDE-1 uridylates risiRNA. a Deep sequencing of total small RNAs of N2 and cde-1 mutant. The red dashed line indicates risiRNAs. b Deep sequencing of Argonaute-associated siRNAs in the indicated animals. c Number of uridylated NRDE-3-associated risiRNAs in the indicated animals. d risiRNA elicited nucleolar accumulation of NRDE-3 in cde-1 mutants. Images of C. elegans embryos of the indicated genotypes. White arrows, nucleolus

Full size image

To test whether risiRNAs bind to Argonaute proteins in addition to NRDE-3, we analyzed HRDE-1 and WAGO-1-bound small RNAs in the young adult animals. HRDE-1 and WAGO-1 were immunoprecipitated from the control animals and the cde-1(tm936) mutant animals. Small RNAs were isolated and deep sequenced in the 5′-phosphate-independent method. In cde-1 mutants, the amount of risiRNAs bound to HRDE-1 and WAGO-1 increased 9.9- and 1.6-fold, respectively, compared to those bound in wild-type animals (Fig. 2b). The NRDE-3-, HRDE-1-, and WAGO-1-bound small RNAs still exhibited the characteristics of 22G-RNAs, which is 22 nt in length and starts with 5′ guanidine in the mutants (Additional file 2: Fig. S2). A similar increase in risiRNA was observed in WAGO-4-bound risiRNAs in cde-1 mutants [8]. CDE-1 adds untemplated uracil to the 3′-ends of CSR-1- and WAGO-4-bound siRNAs. We analyzed the NRDE-3-bound risiRNAs and found that there was a loss of the added untemplated uracil in cde-1 mutants (Fig. 2c).

Small RNAs associate with NRDE-3 and guide NRDE-3 to the target nuclear nucleic acids. In the presence of risiRNA, NRDE-3 accumulated in the nucleoli of cde-1 mutants (Fig. 2d). FIB-1 in C. elegans is encoded by an ortholog of the genes encoding human fibrillarin and Saccharomyces cerevisiae Nop1p [28, 29]. FIB-1 localizes to the nucleolus in embryos. This result suggested that NRDE-3 translocated to the nucleoli and risiRNAs may thereby silence rRNAs in the nucleoli due to double depletions of cde-1 and eri-1.

CDE-1 interacts with SUSI-1(ceDIS3L2) in the germline

To further understand the function of CDE-1, we constructed a GFP::3×FLAG tagged cde-1p::CDE-1::GFP::3×FLAG transgene (abbreviated as CDE-1::GFP) using the MosSCI technology. CDE-1 was expressed in the germline cells at all developmental stages (Additional file 3: Fig. S3 A). CDE-1 localized in the cytoplasm and accumulated in the perinuclear region exhibiting distinct foci in the germline of adult animals. We crossed the CDE-1::GFP strain with the P-granule marker strain mRuby::PGL-1 and found that CDE-1 largely colocalized with the P-granule marker PGL-1 (Fig. 3a).

Fig. 3
figure 3

CDE-1 interacts with SUSI-1(ceDIS3L2) in the germline. a CDE-1 largely colocalized with the P-granule marker PGL-1. Images show the germline cells of young adult animals. b A summary of the top ten putative interacting proteins identified by CDE-1 immunoprecipitation followed by mass spectrometry. WD score: A scoring metrix for identifying high-confidence candidate interacting proteins (HCIPs) http://besra.hms.harvard.edu/ipmsmsdbs/cgi-bin/tutorial.cgi. c The protein-protein interaction of CDE-1 and SUSI-1(ceDIS3L2) was assayed by coimmunoprecipitation followed by western blotting with the indicated antibodies. d SUSI-1(ceDIS3L2) accumulated in the cytoplasm. Images of CDE-1 and SUSI-1 expression in the germline cells at young adult stage

Full size image

We further searched for proteins that interact with CDE-1. We used coimmunoprecipitation followed by mass spectrometry (IP-MS) to identify proteins that potentially interact with CDE-1. Strikingly, we identified SUSI-1(ceDis3L2) (Fig. 3B; Additional file 3: Fig. S3 B). SUSI-1(ceDIS3L2) is a 3′ to 5′ exoribonuclease that degrades oligouridylated RNAs. In susi-1 mutants, both risiRNAs and oligouridylated rRNAs accumulated [20]. To confirm the protein-protein interaction between CDE-1 and SUSI-1(ceDIS3L2), we generated an antibody targeting SUSI-1(ceDIS3L2). CDE-1::GFP was immunoprecipitated by anti-FLAG antibody. Western blotting of the pelleted proteins with SUSI-1(ceDIS3L2) antiserum confirmed the protein-protein interaction between CDE-1 and SUSI-1(ceDIS3L2) in vivo (Fig. 3c). We then generated single-copy 3×FLAG::GFP::SUSI-1 and CDE-1::mCherry transgenes and found that SUSI-1(ceDIS3L2) accumulated in the cytoplasm of the germline cells (Fig. 3d).

Therefore, we conclude that CDE-1 and SUSI-1(ceDIS3L2) likely function as a protein complex to suppress risiRNAs production.

CDE-1 is involved in uridylation of rRNA

Previously, we showed that SUSI-1(ceDIS3L2) degrades oligouridylated rRNAs and suppresses the production of risiRNA [20]. To examine whether CDE-1 uridylates rRNAs, a 3′ tail-seq method was used to detect the oligouridylation of rRNA at the 3′-tail in the indicated genotypes (Fig. 4a). Total RNA was isolated from L3-staged control and indicated animals, and then libraries were prepared by PCR amplification with a corresponding rRNA primer and a primer targeting the linker, which were followed by high-throughput sequencing (Fig. 4a).

Fig. 4
figure 4

CDE-1 is involved in the 3′-end uridylation of 26S and 5.8S rRNAs. a A schematic of the rRNA tail-seq method. b, d Tail-seq data of 26S rRNAs from indicated animals at L3 stage. c, e Tail-seq data of 5.8S rRNAs from indicated animals at L3 stage. The numbers of reads with untemplated oligouridylation at the 3′-ends are indicated. Data are presented as the mean ± SD (n = 3, biological replicates). ns, not significant. *P < 0.05, **P < 0.01 (two-tailed Student’s t test)

Full size image

The 3′-end of 26S rRNA was extensively modified by all four nucleotides compared to the annotated rRNA sequence [20]. We tried to detect the 3′-ends of 26S and 5.8S rRNA. We found that both 26S rRNA (Fig. 4b) and 5.8S rRNA (Fig. 4c) are well processed at the 3′-tails as the 3′-end nucleic acid of most RNAs is the same. Although we did not detect a dramatic change in the nontemplated addition of a single nucleotide, we observed a modest depletion of oligouridylation at the 3′-tail of 26S rRNA, comparing cde-1(tm936) to wild-type N2 animals at 20 °C. The depletion of oligouridylation of 26 rRNA can be rescued by a introduction of the CDE-1::GFP transgene (Fig. 4d). Previously, we have noticed that risiRNA was enriched in cold-shocked worms [20]. Here, we discovered a significant increase of oligouridylation at the 3′-tail of 26S rRNA, comparing wild-type N2 animals at 20 °C to cold-shocked N2 worms at 4 °C for 12 h. Meanwhile, cde-1 mutation blocked the increase triggered by the cold shock treatment (Fig. 4d). We also noticed a significant increase of oligouridylation at the 3′-tail of 26S rRNA, comparing susi-1(ust1) to wild-type N2 animals at 20 °C (Fig. 4d). Furthermore, to uncover how CDE-1 and SUSI-1(ceDIS3L2) affect oligouridylation at the 3′-end of rRNA simultaneously, we knocked down susi-1 in cde-1(tm936) mutants, as these two genes are too close on the genome to be genetically manipulated. We detected a significant decrease of susi-1 mRNA level (Additional file 4: Fig. S4). However, there is no change of the oligouridylation at the 3′-tail of 26S rRNA, comparing to the untreated cde-1(tm936) worms.

As for 5.8S rRNA, we detected a dramatic change in the nontemplated addition of a single U nucleotide, which was accompanied by a significant increase of oligouridylation at the 3′-tail, comparing wild-type N2 animals at 20 °C to cold-shocked N2 worms at 4 °C. In the same way, depletion of cde-1 blocked the increase of mono- or oligo-uridylation triggered by cold shock. Similarly, the change tendency of uridylation at the 3′-tail of 5.8S rRNA in the indicated genotype or under cold shock treatment is consistent with that of 26S rRNA (Fig. 4e).

Notably, it is obvious that CDE-1 prefers to add 3–6 Us to 3′-end of 26S rRNA and add 1–6 U(s) to 3′-tail of 5.8S rRNA, which may lead to degradation by SUSI-1(ceDIS3L2). This result indicates that SUSI-1(ceDIS3L2) may recognize, bind and process shorter oligoU uridylated rRNA, which is not consistent with the substrate preference (10–14 uridines or greater) of mouse Dis3l2 in the Lin28-let-7 pathway [22, 30].

Taken together, these data suggest that cold shock leads to uridylation at the 3′-tail of rRNA, and CDE-1 is involved in uridylating 26S and 5.8S rRNAs.

SUSI-1(ceDIS3L2) is required for the inheritance of RNAi

It was previously shown that CDE-1 is required for the inheritance of RNAi by uridylating WAGO-4-associated siRNAs [8, 31]. Since CDE-1 interacts with SUSI-1(ceDIS3L2), we then asked whether susi-1 was also required for the inheritance of RNAi. We used a germline-expressed mex-5p::GFP::H2B (abbreviated as GFP::H2B) transgene as a reporter, which can inherit RNAi-induced gene silencing for multiple generations. Both hrde-1 and cde-1 were not required for exogenous gfp dsRNA to silence the GFP::H2B transgene in the parental generation, but they were essential for silencing in the F1 to F3 generations (Fig. 5). Similarly, susi-1(ceDis3L2) was not required for exogenous gfp dsRNA to silence the GFP::H2B transgene in the P0 generation but was necessary for silencing in F1 to F3 progeny. We conclude that susi-1(ceDis3L2) is required for the inheritance of RNAi.

Fig. 5
figure 5

Both CDE-1 and SUSI-1(ceDIS3L2) are required for the inheritance of RNAi. a mex-5p::GFP::H2B transgenic animals were exposed to bacteria expressing gfp dsRNA. F1 embryos were isolated and grown on control bacteria in the absence of further gfp dsRNA treatment. GFP expression in the indicated animals was imaged in the germline and oocytes. b The percentage of P0 to F3 animals expressing GFP was counted

Full size image

Discussion

Misprocessed rRNAs are usually detected and degraded by surveillance machinery during ribosome biogenesis [13, 14, 23, 32]. Previously, our lab identified a class of risiRNAs that downregulate pre-rRNAs through the nuclear RNAi pathway to suppress the accumulation of erroneous rRNAs. We identified a number of broadly conserved genes that are involved in rRNA processing and maturation. The depletion of these genes leads to an increase in risiRNAs. Thereafter, these genes are named suppressor of siRNA (susi) [20, 24]. Among them, SUSI-1(ceDIS3L2) plays a vital role in the 3′-5′ degradation of oligouridylated rRNA fragments [20]. In this work, we further found that CDE-1 uridylates the 3′-end of 26S and 5.8S rRNAs and may recruit SUSI-1(ceDIS3L2) through protein-protein interactions. Therefore, we conclude that cde-1 is a new susi gene and suppresses the generation of risiRNAs.

Uridylation of the 3′-end of RNAs plays important functions in determining the fate of RNA [33, 34]. For example, uridylation is an intrinsic step in the maturation of noncoding RNAs, including the U6 spliceosomal RNA or mitochondrial guide RNAs in trypanosomes [35]. Uridylation can also switch specific miRNA precursors from a degradative to a processing mode. This switch depends on the number of uracils added and is regulated by the cellular context [36, 37]. However, the typical consequence of uridylation is accelerating the RNA degradation [21, 38]. In this work, we showed that CDE-1 can uridylate 26S and 5.8S rRNAs and recruit the 3′-5′ exoribonuclease SUSI-1(ceDIS3L2), which may further promote the degradation of oligouridylated rRNAs. In the absence of either CDE-1 or SUSI-1(ceDIS3L2), erroneous rRNAs will accumulate in cells, which thereafter recruit the RNA-dependent RNA polymerases, including RRF-1 and RRF-2, to initiate risiRNA production (Fig. 6). risiRNAs then bind to both nuclear and cytoplasmic Argonaute proteins and silence rRNAs through both nuclear and cytoplasmic RNAi machinery. Therefore, risiRNA and the RNAi machinery, together with exoribonucleases, act to avoid the accumulation of potentially harmful or unnecessary erroneous rRNA transcripts [14, 15, 17, 18, 32, 39, 40]. 3′-end modifications play important roles in regulating the stability of siRNAs via distinct mechanisms as well. For example, methylation of the 3′-end inhibits uridylation and correlates with increased steady state levels of small RNAs [41, 42]. In contrary, 3′ terminal uridylation may promote the degradation of siRNA [9, 43]. CDE-1 uridylates endogenous siRNAs and modulates their binding affinity to CSR-1 and WAGO-4 [8, 9]. PUP-2 has been reported to target let-7 miRNA [11, 37]. Although PUP-3 has been validated as uridyl transferase, its targets are still unclear. Here, we found that CDE-1, but not PUP-2 or PUP-3, are engaged in suppressing risiRNA production. How these PUPs recognize their specific targets is still an enigma.

Fig. 6
figure 6

A working model of risiRNA biogenesis in C. elegans. The erroneous cellular rRNAs are scrutinized and suppressed through a number of mechanisms. Erroneous rRNAs are uridylated by CDE-1 and degraded by exoribonucleases such as SUSI-1(ceDis3L2). The disruption of CDE-1 or SUSI-1(ceDis3L2) results in the accumulation of erroneous rRNAs that thereafter recruit RdRPs to synthesize risiRNA. A risiRNA-mediated feedback loop silences rRNA expression through RNAi machinery and compensates for the disruption of the degradation of erroneous rRNA transcripts

Full size image

Additional questions remain as to how and why erroneous rRNAs could be recognized by CDE-1. Our previous work found that either the modification errors or processing errors of rRNAs trigger the generation of risiRNAs [24]. How these different kinds of errors are sensed and scrutinized is still unknown. Deciphering the intricate interaction network of CDE-1 or other TUTases is key to fully understanding the effect of RNA uridylation. In addition, CDE-1 was previously reported required for RNAi inheritance [8, 31]. The underlying mechanism remains unclear. Our previous data suggested that CDE-1 may mediate RNAi inheritance by regulating the binding of 22GRNAs to WAGO-4 [8]. Here, we found that CDE-1 interacted with SUSI-1(ceDIS3L2), another protein required for the inheritance of RNAi. Further elucidating the function of SUSI-1(ceDIS3L2) and CDE-1 will shed light on the mechanism of RNAi inheritance.

Conclusions

RNA uridylation is a potent and widespread posttranscriptional regulator of gene expression. The untemplated terminal polyuridylation has a decisive impact on RNA’s fate. In this article, we further decipher the molecular mechanism of risiRNA generation in C. elegans. We provide genetic, cell biological, and biochemical evidence documenting the function of CDE-1, which uridylates rRNAs at 3′-ends. By using IP-MS technology, we found that CDE-1 interacts with SUSI-1(ceDIS3L2), a 3′-5′ exoribonuclease that we previously found to suppress risiRNA production. CDE-1 also uridylates Argonaute-associated risiRNAs. Interestingly, both CDE-1 and SUSI-1(ceDIS3L2) promote RNAi inheritance. In addition, this study sheds new light on a complicated surveillance network by combining uridylation, degradation, and RNAi-mediated gene silencing to maintain rRNA homeostasis.

Methods

Strains

Bistol strain N2 was used as the standard wild-type strain. All strains were grown at 20 °C unless otherwise specified. The strains used in this study were listed in Additional file 5: Table S1.

Quantification of the subcellular location of NRDE-3

The subcellular localization of NRDE-3 was quantified as described previously [20]. Images were collected on a Leica DM4B microscope.

Quantitative RT-PCR

RNA was isolated from the indicated animals and subjected to DNase I digestion (Thermo Fisher). cDNA was generated from the isolated RNA using a GoScript™ Reverse Transcription System (Promega) according to the vendor’s protocol. qPCR was performed using a MyIQ2 real-time PCR system (Bio-Rad) with an AceQ SYBR Green Master mix (Vazyme). The primers used in RT-qPCR were listed in Additional file 6: Table S2. eft-3 mRNA was used as an internal control for sample normalization. Data analysis was performed using a comparative threshold cycle (ΔΔCT) approach.

Brood size

Synchronized L3 worms were individually placed onto fresh NGM plates, and the progeny numbers were scored.

Construction of plasmids and transgenic strains

For CDE-1::GFP, a cde-1 promoter and CDS region were PCR-amplified with the primers 5′-TACGACTCACTAGTGGGCAGgacgtgggacataaacgaagaaag-3′ and 5′-ATAGCTCCACCTCCACCTCCTTTGTTGTACGAGCGATGATAG-3′ from N2 genomic DNA. A GFP::3×FLAG region was PCR-amplified with the primers 5′-GGAGGTGGAGGTGGAGCTATGAGTAAAGGAGAAGAAC-3′ and 5′-TCACTTGTCATCGTCATCCT-3′ from plasmid pSG085. The CDE-1 3′ UTR (untranslated region) was PCR-amplified with the primers 5′- ACAAGGATGACGATGACAAGTAAattctctccacccattcac-3′ and 5′- CTACGTAATACGACTCACTTaactgatcggttgcttctctcac-3′ from N2 genomic DNA. A ClonExpress MultiS One-step Cloning Kit (Vazyme, C113–02) was used to insert the CDE-1::GFP::3×FLAG fusion gene into the pCFJ151 vector. The transgene was integrated into C. elegans chromosome II by the MosSCI method [44]. Using the same method, the CDE-1::mCherry fusion gene was integrated into C. elegans chromosome V.

The primers used for dual-sgRNA-directed CRISPR/Cas9-mediated cde-1 gene deletion were 5′-TCCGGATAGTGATTACAATG-3′ and 5′-GGTATTATGTTGAACGACAT-3′.

For 3×FLAG::GFP::SUSI-1, the predicted susi-1 promoter was PCR-amplified with the primers 5′-TACGACTCACTAGTGGGCAGtatcagggagattctgctgtg-3′ and 5′- tcatggtctttgtagtccatACTTTCAACTGCTGACATctag-3′ from N2 genomic DNA. The 3×FLAG::GFP coding region was PCR amplified from plasmid pSG085 with the primers 5′-AGCTCTTCCTATGGACTACAAAGACCATGAC-3′ and 5′- ATAGCTCCACCTCCACCTCCTTTGTATAGTTCATCCATGCC-3′. The susi-1 coding region and the predicted 3′ UTR were then amplified by PCR from N2 genomic DNA with primers 5′-AAGGAGGTGGAGGTGGAGCTATGTCAGCAGTTGAAAGTCCCG-3′ and 5′-CTACGTAATACGACTCACTTGTGTGGATTAACACAGCCAATTG-3′ from N2 genomic DNA. The ClonExpress MultiS One-step Cloning Kit (Vazyme, C113-02) was used to insert the 3×FLAG::GFP::SUSI-1 fusion gene into the pCFJ151 vector. The transgene was integrated into C. elegans chromosome II by the MosSCI system.

RNA immunoprecipitation (RIP)

RIP experiments were performed as previously described with hypochlorite-isolated embryos of indicated animals [20]. The embryos were sonicated in lysis buffer (20 mM Tris-HCl (pH 7.5), 200 mM NaCl, 2.5 mM MgCl2, and 0.5% NP-40), precleared with protein G-agarose beads (Roche), and incubated with anti-FLAG M2 agarose beads (Sigma #A2220). The beads were washed extensively, and 3×FLAG::GFP-tagged protein and associated RNAs were eluted with 100 μg/mL 3×FLAG peptide (Sigma). The eluates were incubated with TRIzol reagent (Invitrogen), which was followed by isopropanol precipitation. Then, small RNAs were quantified by deep sequencing.

Deep sequencing of small RNAs and bioinformatic analysis

Total RNAs and the Argonaute-associated RNAs were isolated from the indicated animals and subjected to small RNA deep sequencing using an Illumina platform (Novogene Bioinformatics Technology Co., Ltd.), as previously described [20].

For Argonaute-associated RNAs, synchronized worms were sonicated in sonication buffer (20 mM Tris-HCl,pH 7.5, 200 mM NaCl, 2.5 mM MgCl2, and 0.5% NP40). The eluates were incubated with TRIzol reagent and then precipitated with isopropanol. The precipitated RNA was treated with FastAP Thermosensitive Alkaline Phosphatase (Thermo Scientific), re-extracted with TRIzol, and treated with T4 Polynucleotide Kinase (T4 PNK, Thermo Scientific) in the presence of 1 mM ATP before library construction.

Small RNAs were subjected to deep sequencing using an Illumina platform (Novogene Bioinformatics Technology Co., Ltd.). Briefly, small RNAs ranging from 18 to 30 nt were gel-purified and ligated to a 3′ adaptor (5′-pUCGUAUGCCGUCUUCUGCUUGidT-3′; p, phosphate; idT, inverted deoxythymidine); and a 5′ adaptor (5′-GUUCAGAGUUCUACAGUCCGACGAUC-3′), respectively. The ligation products were gel-purified, reverse transcribed, and amplified using an Illumina sRNA primer set (5′-CAAGCAGAAGACGGCATACGA-3′; 5′-AATGATACGGCGACCACCGA-3′). The samples were then sequenced using an Illumina HiSeq platform.

The Illumina-generated raw reads were first filtered to remove adaptors, low-quality tags, and contaminants to obtain clean reads by Novogene. Clean reads ranging from 18 to 30 nt were mapped to the transcriptome assembly WS243 using Bowtie2 with default parameters. The number of reads targeting each transcript were counted by custom Perl scripts. The number of total reads mapped to the genome minus the number of total reads corresponded to sense rRNA transcripts (5S, 5.8S, 18S, and 26S), which was used as the normalization number, to exclude the possible degradation fragments of sense rRNAs.

Proteomic analysis

Proteomic analysis was conducted as previously described [45]. Briefly, mixed-stage transgenic worms expressing CDE-1::GFP were resuspended in equal volumes of 2× lysis buffer (50 mM Tris-HCl pH 8.0, 300 mM NaCl, 10% glycerol, 1% Triton X-100, Roche®cOmplete EDTA-free Protease Inhibitor Cocktail, 10 mM NaF, and 2 mM Na3VO4), and lysed in a FastPrep-24 5G homogenizer. The lysate supernatant was incubated with anti-GFP antibody, which was linked to beads, for 1 h at 4 °C. The beads were then washed three times with cold lysis buffer. The GFP immunoprecipitates were eluted with chilled elution buffer (100 mM glycine-HCl, pH 2.5). Approximately 1/8 of the eluates were subjected to western blotting analysis. The rest of the eluates were precipitated with TCA or cold acetone and dissolved in 100 mM Tris (pH 8.5), with 8 M urea. The proteins were reduced with TCEP, alkylated with IAA, and finally digested with trypsin at 37 °C overnight. LC-MS/MS analysis of the resulting peptides and MS data processing approaches were conducted as previously described [46]. A WD scoring matrix was used to identify high-confidence candidate interacting proteins.

Coimmunoprecipitation analysis

The lysates of transgenic worms were prepared using RIP lysis buffer (50 mM Tris (pH 7.4), 150 mM NaCl, 1% NP-40, 0.1% SDS, 1 mM EDTA, 0.5% sodium deoxycholate, and protease inhibitors (Thermo)). Immunoprecipitations with anti-FLAG® M2 affinity gel (a2220, Sigma) or agarose beads (ab193255, Abcam) with anti-GFP antibody (ab290, Abcam) and anti-SUSI-1 antibody (lot number 20121105, Abmart) were performed at 4 °C overnight. Protein complexes were eluted by boiling in 2× SDS loading buffer. Anti-GFP, anti-SUSI-1 and anti-Actin (Servicebio GB12001) antibodies that were used for western blots were diluted to 1:2000, 1:500, and 1:5000, respectively.

rRNA 3′ tail-seq

rRNA tail-seq was conducted as described previously [20]. Briefly, total RNA were extracted from L3 larva, digested by DNase I, and then ligated to the following 3′ RNA linkers with T4 RNA ligase (Thermo #EL0021) (1 μg total RNA, 2 μL 3′ RNA linker (10 μM), 1 μL 10× T4 RNA ligation buffer, 2 μL T4 RNA ligase) by incubating at 37 °C for 30 min.

3′ RNA linker-1:

5′-pGATCCACACTCGGGCACCAAGGATTTAACCGCGAATTCCAGC-NH2–3′ (the underlined sequence served as a barcode for sample labeling).

3′ RNA linker-2:

5′-pCGACACACTCGGGCACCAAGGATTTAACCGCGAATTCCAGC-NH2–3′.

3′ RNA linker-3:

5′-pGTACCACACTCGGGCACCAAGGATTTAACCGCGAATTCCAGC-NH2–3′.

The RNAs were reverse transcribed with the following primer:

Universal 3′ linker RT:

5′-GCTGGAATTCGCGGTTAAATCCTTGGTGCCCGAGTGT-3′. The cDNAs were PCR amplified (16 cycles) with the primers 26S rRNA-F: 5′-CAGATCACTCTGGTTCAATGTC-3′ and universal 3′ linker RT primer, or with the primers 5.8S rRNA-F: 5′-GGTTGCATCGAGTATCGATGAA-3′ and universal 3′ linker RT primer, gel purified and then deep sequenced using an Illumina platform, according to the manufacturer′s instructions, by Novogene (Beijing, China). The number of reads with distinct 3′-end modifications was counted by custom Perl scripts. Three biological replicates were conducted in each genotype or treatment.

RNAi inheritance assay

Synchronized L1 animals of the indicated genotypes were exposed to bacteria expressing gfp dsRNA. F1 embryos were collected by hypochlorite/NaOH treatment and grown on OP50 bacteria. The GFP expression levels in both the parental generation (P0) and the progeny (F1–F3) were visualized and scored. Images were collected with a Leica DM4B microscope system.

Statistics

Bar graphs with error bars represent the mean and SD. All of the experiments were conducted with independent C. elegans animals for the indicated N replicates. Statistical analysis was performed with two-tailed Student’s t tests or unpaired Wilcoxon tests. The threshold for Student’s t test P values was set to 0.05 or 0.01.

Availability of data and materials

All raw and normalized sequencing data have been deposited to Gene Expression Omnibus under submission number GSE139530 [47] and GSE156000 [48].

References

  1. Blahna MT, Jones MR, Quinton LJ, Matsuura KY, Mizgerd JP. Terminal uridyltransferase enzyme Zcchc11 promotes cell proliferation independent of its uridyltransferase activity. J Biol Chem. 2011;286(49):42381–9.

    CAS  PubMed  PubMed Central  Google Scholar 

  2. Hagan JP, Piskounova E, Gregory RI. Lin28 recruits the TUTase Zcchc11 to inhibit let-7 maturation in mouse embryonic stem cells. Nat Struct Mol Biol. 2009;16(10):1021–5.

    CAS  PubMed  PubMed Central  Google Scholar 

  3. Jones MR, Quinton LJ, Blahna MT, Neilson JR, Fu S, Ivanov AR, Wolf DA, Mizgerd JP. Zcchc11-dependent uridylation of microRNA directs cytokine expression. Nat Cell Biol. 2009;11(9):1157–63.

    CAS  PubMed  PubMed Central  Google Scholar 

  4. Le Pen J, Jiang H, Di Domenico T, Kneuss E, Kosalka J, Leung C, Morgan M, Much C, Rudolph KLM, Enright AJ, et al. Terminal uridylyltransferases target RNA viruses as part of the innate immune system. Nat Struct Mol Biol. 2018;25(9):778–86.

    PubMed  PubMed Central  Google Scholar 

  5. Warkocki Z, Krawczyk PS, Adamska D, Bijata K, Garcia-Perez JL, Dziembowski A. Uridylation by TUT4/7 restricts retrotransposition of human LINE-1s. Cell. 2018;174(6):1537.

    CAS  PubMed  PubMed Central  Google Scholar 

  6. Yeo J, Kim VN. U-tail as a guardian against invading RNAs. Nat Struct Mol Biol. 2018;25(10):903–5.

    CAS  PubMed  Google Scholar 

  7. Kwak JE, Wickens M. A family of poly(U) polymerases. RNA. 2007;13(6):860–7.

    CAS  PubMed  PubMed Central  Google Scholar 

  8. Xu F, Feng XZ, Chen XY, Weng CC, Yan Q, Xu T, Hong MJ, Guang SH. A cytoplasmic Argonaute protein promotes the inheritance of RNAi. Cell Rep. 2018;23(8):2482–94.

    CAS  PubMed  Google Scholar 

  9. van Wolfswinkel JC, Claycomb JM, Batista PJ, Mello CC, Berezikov E, Ketting RF. CDE-1 affects chromosome segregation through uridylation of CSR-1-bound siRNAs. Cell. 2009;139(1):135–48.

    PubMed  Google Scholar 

  10. Claycomb JM, Batista PJ, Pang KM, Gu W, Vasale JJ, van Wolfswinkel JC, Chaves DA, Shirayama M, Mitani S, Ketting RF, et al. The Argonaute CSR-1 and its 22G-RNA cofactors are required for holocentric chromosome segregation. Cell. 2009;139(1):123–34.

    CAS  PubMed  PubMed Central  Google Scholar 

  11. Lehrbach NJ, Armisen J, Lightfoot HL, Murfitt KJ, Bugaut A, Balasubramanian S, Miska EA. LIN-28 and the poly(U) polymerase PUP-2 regulate let-7 microRNA processing in Caenorhabditis elegans. Nat Struct Mol Biol. 2009;16(10):1016–20.

    CAS  PubMed  PubMed Central  Google Scholar 

  12. Li Y, Maine EM: The balance of poly(U) polymerase activity ensures germline identity, survival and development in Caenorhabditis elegans. Development 2018, 145(19):dev165944. https://doi.org/10.1242/dev.165944.

  13. Lafontaine DLJ. Noncoding RNAs in eukaryotic ribosome biogenesis and function. Nat Struct Mol Biol. 2015;22(1):11–9.

    CAS  PubMed  Google Scholar 

  14. Henras AK, Plisson-Chastang C, O'Donohue MF, Chakraborty A, Gleizes PE. An overview of pre-ribosomal RNA processing in eukaryotes. Wiley Interdiscip Rev RNA. 2015;6(2):225–42.

    CAS  PubMed  Google Scholar 

  15. Lafontaine DL. A ‘garbage can’ for ribosomes: how eukaryotes degrade their ribosomes. Trends Biochem Sci. 2010;35(5):267–77.

    CAS  PubMed  Google Scholar 

  16. Thoms M, Thomson E, Bassler J, Gnadig M, Griesel S, Hurt E. The exosome is recruited to RNA substrates through specific adaptor proteins. Cell. 2015;162(5):1029–38.

    CAS  PubMed  Google Scholar 

  17. Vanacova S, Stefl R. The exosome and RNA quality control in the nucleus. EMBO Rep. 2007;8(7):651–7.

    CAS  PubMed  PubMed Central  Google Scholar 

  18. Houseley J, LaCava J, Tollervey D. RNA-quality control by the exosome. Nat Rev Mol Cell Biol. 2006;7(7):529–39.

    CAS  PubMed  Google Scholar 

  19. Lubas M, Damgaard CK, Tomecki R, Cysewski D, Jensen TH, Dziembowski A. Exonuclease hDIS3L2 specifies an exosome-independent 3 '-5 ' degradation pathway of human cytoplasmic mRNA. EMBO J. 2013;32(13):1855–68.

    CAS  PubMed  PubMed Central  Google Scholar 

  20. Zhou XF, Feng XZ, Mao H, Li M, Xu F, Hu K, Guang SH. RdRP-synthesized antisense ribosomal siRNAs silence pre-rRNA via the nuclear RNAi pathway. Nature Structural Mole Biol. 2017;24(3):258.

    CAS  Google Scholar 

  21. Ustianenko D, Pasulka J, Feketova Z, Bednarik L, Zigackova D, Fortova A, Zavolan M, Vanacova S. TUT-DIS3L2 is a mammalian surveillance pathway for aberrant structured non-coding RNAs. EMBO J. 2016;35(20):2179–91.

    CAS  PubMed  PubMed Central  Google Scholar 

  22. Faehnle CR, Walleshauser J, Joshua-Tor L. Mechanism of Dis3l2 substrate recognition in the Lin28-let-7 pathway. Nature. 2014;514(7521):252–6.

    CAS  PubMed  PubMed Central  Google Scholar 

  23. Pirouz M, Munafo M, Ebrahimi AG, Choe J, Gregory RI. Exonuclease requirements for mammalian ribosomal RNA biogenesis and surveillance. Nat Struct Mol Biol. 2019;26(6):490–500.

    CAS  PubMed  PubMed Central  Google Scholar 

  24. Zhu C, Yan Q, Weng C, Hou X, Mao H, Liu D, Feng X, Guang S. Erroneous ribosomal RNAs promote the generation of antisense ribosomal siRNA. Proc Natl Acad Sci U S A. 2018;115(40):10082–7.

    CAS  PubMed  PubMed Central  Google Scholar 

  25. Zhou X, Chen X, Wang Y, Feng X, Guang S. A new layer of rRNA regulation by small interference RNAs and the nuclear RNAi pathway. RNA Biol. 2017;14(11):1492–8.

    PubMed  PubMed Central  Google Scholar 

  26. Yan Q, Zhu C, Guang S, Feng X. The functions of non-coding RNAs in rRNA regulation. Front Genet. 2019;10:290.

    CAS  PubMed  PubMed Central  Google Scholar 

  27. Guang S, Bochner AF, Pavelec DM, Burkhart KB, Harding S, Lachowiec J, Kennedy S. An Argonaute transports siRNAs from the cytoplasm to the nucleus. Science. 2008;321(5888):537–41.

    CAS  PubMed  PubMed Central  Google Scholar 

  28. Yi YH, Ma TH, Lee LW, Chiou PT, Chen PH, Lee CM, Chu YD, Yu H, Hsiung KC, Tsai YT, et al. A genetic cascade of let-7-ncl-1-fib-1 modulates nucleolar size and rRNA Pool in Caenorhabditis elegans. PLoS Genet. 2015;11(10):e1005580.

    PubMed  PubMed Central  Google Scholar 

  29. Lee LW, Lee CC, Huang CR, Lo SJ. The nucleolus of Caenorhabditis elegans. J Biomed Biotechnol. 2012;2012:601274.

    PubMed  PubMed Central  Google Scholar 

  30. Chang H, Triboulet R, Thornton JE, Gregory RIJN: A role for the Perlman syndrome exonuclease Dis3l2 in the Lin28–let-7 pathway. 2013, 497(7448):244–248.

  31. Spracklin G, Fields B, Wan G, Becker D, Wallig A, Shukla A, Kennedy S. The RNAi inheritance machinery of Caenorhabditis elegans. Genetics. 2017;206(3):1403–16.

    CAS  PubMed  PubMed Central  Google Scholar 

  32. Schmidt K, Butler JS. Nuclear RNA surveillance: role of TRAMP in controlling exosome specificity. Wiley Interdiscip Rev RNA. 2013;4(2):217–31.

    CAS  PubMed  PubMed Central  Google Scholar 

  33. Menezes MR, Balzeau J, Hagan JP. 3 ' RNA uridylation in epitranscriptomics, gene regulation, and disease. Front Mol Biosci. 2018;5.

  34. Lee M, Kim B, Kim VN. Emerging roles of RNA modification: m (6) A and U-tail. Cell. 2014;158(5):980–7.

    CAS  PubMed  Google Scholar 

  35. Trippe R, Guschina E, Hossbach M, Urlaub H, Luhrmann R, Benecke BJ. Identification, cloning, and functional analysis of the human U6 snRNA-specific terminal uridylyl transferase. Rna-a Publication of the Rna Society. 2006;12(8):1494–504.

    CAS  Google Scholar 

  36. De Almeida C, Scheer H, Zuber H, Gagliardi D: RNA uridylation: a key posttranscriptional modification shaping the coding and noncoding transcriptome. Wiley Interdisciplinary Reviews-Rna 2018, 9(1). https://doi.org/10.1002/wrna.1440.

  37. Heo I, Ha M, Lim J, Yoon MJ, Park JE, Kwon SC, Chang H, Kim VN. Mono-uridylation of pre-microRNA as a key step in the biogenesis of group II let-7 microRNAs. Cell. 2012;151(3):521–32.

    CAS  PubMed  Google Scholar 

  38. Pirouz M, Du P, Munafo M, Gregory RI. Dis3l2-mediated decay is a quality control pathway for noncoding RNAs. Cell Rep. 2016;16(7):1861–73.

    CAS  PubMed  PubMed Central  Google Scholar 

  39. Pena C, Hurt E, Panse VG. Eukaryotic ribosome assembly, transport and quality control. Nat Struct Mol Biol. 2017;24(9):689–99.

    CAS  PubMed  Google Scholar 

  40. Karbstein K. Quality control mechanisms during ribosome maturation. Trends Cell Biol. 2013;23(5):242–50.

    CAS  PubMed  PubMed Central  Google Scholar 

  41. Ren G, Xie M, Zhang S, Vinovskis C, Chen X, Yu B. Methylation protects microRNAs from an AGO1-associated activity that uridylates 5′ RNA fragments generated by AGO1 cleavage. Proc Natl Acad Sci U S A. 2014;111(17):6365–70.

    CAS  PubMed  PubMed Central  Google Scholar 

  42. Kamminga LM, Luteijn MJ, den Broeder MJ, Redl S, Kaaij LJ, Roovers EF, Ladurner P, Berezikov E, Ketting RF. Hen1 is required for oocyte development and piRNA stability in zebrafish. EMBO J. 2010;29(21):3688–700.

    CAS  PubMed  PubMed Central  Google Scholar 

  43. Ibrahim F, Rymarquis LA, Kim EJ, Becker J, Balassa E, Green PJ, Cerutti H. Uridylation of mature miRNAs and siRNAs by the MUT68 nucleotidyltransferase promotes their degradation in Chlamydomonas. Proc Natl Acad Sci U S A. 2010;107(8):3906–11.

    CAS  PubMed  PubMed Central  Google Scholar 

  44. Frokjaer-Jensen C, Davis MW, Sarov M, Taylor J, Flibotte S, LaBella M, Pozniakovsky A, Moerman DG, Jorgensen EM. Random and targeted transgene insertion in Caenorhabditis elegans using a modified Mos1 transposon. Nat Methods. 2014;11(5):529–34.

    PubMed  PubMed Central  Google Scholar 

  45. Zeng C, Weng C, Wang X, Yan YH, Li WJ, Xu D, Hong M, Liao S, Dong MQ, Feng X, et al. Functional proteomics identifies a PICS complex required for piRNA maturation and chromosome segregation. Cell Rep. 2019;27(12):3561–72 e3563.

    CAS  PubMed  Google Scholar 

  46. Feng GX, Zhu ZW, Li WJ, Lin QR, Chai YP, Dong MQ, Ou GS. Hippo kinases maintain polarity during directional cell migration in Caenorhabditis elegans. EMBO J. 2017;36(3):334–45.

    CAS  PubMed  Google Scholar 

  47. Wang Y, Weng C, Chen X, Zhou X, Huang X, Yan Y, Zhu C. CDE-1 suppresses the production of risiRNA by coupling polyuridylation and degradation of rRNA. Supplementary Datasets. 2020. NCBI accession GSE139530 https://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?acc=GSE139530.

  48. Wang Y, Weng C, Chen X, Zhou X, Huang X, Yan Y, Zhu C. CDE-1 suppresses the production of risiRNA by coupling polyuridylation and degradation of rRNA. Supplementary Datasets. 2020. NCBI accession GSE156000 https://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?acc=GSE156000.

Download references

Acknowledgements

We would like to thank all donors who participated in the study without whom this work would have not been possible. We are grateful to Drs. Shouhong Guang, Shanhui Liao, Shuai Wei, and the members of the Guang lab for their comments. We are grateful to the International C. elegans Gene Knockout Consortium and the National Bioresource Project for providing the strains. Some strains used in this study were provided by the CGC, which is funded by NIH Office of Research Infrastructure Programs (P40 OD010440).

Funding

This work was supported by grants from the China Postdoctoral Science Foundation (2015 M582006), the Natural Science Foundation of Anhui Province (1608085MC68). Cultivation project of excellent top talents in Colleges and Universities (gxbjZD2020085).

Author information

Author notes

  1. Yun Wang and Chenchun Weng contributed equally to this work.

Affiliations

  1. National Science Center for Physical Sciences at Microscale Division of Molecular & Cell Biophysics, School of Life Sciences, University of Science and Technology of China, Hefei, 230027, Anhui, People’s Republic of China

    Yun Wang, Chenchun Weng, Xiangyang Chen, Xufei Zhou, Xinya Huang & Chengming Zhu

  2. School of Bioengineering, Huainan Normal University, Huainan, 232038, Anhui, People’s Republic of China

    Yun Wang

  3. National Institute of Biological Sciences, Beijing, 102206, People’s Republic of China

    Yonghong Yan

Authors
  1. Yun Wang
    View author publications

    You can also search for this author in PubMed Google Scholar

  2. Chenchun Weng
    View author publications

    You can also search for this author in PubMed Google Scholar

  3. Xiangyang Chen
    View author publications

    You can also search for this author in PubMed Google Scholar

  4. Xufei Zhou
    View author publications

    You can also search for this author in PubMed Google Scholar

  5. Xinya Huang
    View author publications

    You can also search for this author in PubMed Google Scholar

  6. Yonghong Yan
    View author publications

    You can also search for this author in PubMed Google Scholar

  7. Chengming Zhu
    View author publications

    You can also search for this author in PubMed Google Scholar

Contributions

YW, CW, and XZ designed the experiments. YW, CW, XC, and XH performed experiments. YW and CW analyzed the data. YW and CW wrote the manuscript. All authors read and approved the final manuscript.

Corresponding author

Correspondence to Yun Wang.

Ethics declarations

Ethics approval and consent to participate

Not applicable.

Consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interests.

Additional information

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Additional file 1: Figure S1.

risiRNA accumulats in cde-1 mutant and requires rrf-1 and rrf-2. (A) → CDE-1::mCherry was able to redistribute NRDE-3 from the nucleus to the cytoplasm in cde-1(tm936) mutants. The germline and the seam cells of indicated animals at L3 stage were shown. White dashed line shows the border of germline. White arrows, nucleus. (B) → The depletion of pup-2 and pup-3 together was not able to redistribute NRDE-3 from the cytoplasm to the nucleus. The seam cells of indicated animals were shown. The numbers indicated the percentage of animals with nuclear enriched NRDE-3 in seam cells. The number of scored animals is indicated in the parentheses. White arrows, nucleus. (C) → rrf-1 and rrf-2 were required for NRDE-3 nuclear localization when cde-1 is not functional. Images of the representative seam cells were shown. The numbers indicated the percentage of animals with nuclear enriched NRDE-3 in seam cells. The number of scored animals is indicated in the parentheses. White arrows, nucleus. (D) → The depletion of rrf-1 and rrf-2 partially restored the fecundity of eri-1(mg366);cde-1(tm936) animals. Data are presented as the mean ± SD (n = 3, biological replicates). **P < 0.01 (two-tailed Student’s t test).

Additional file 2: Figure S2.

Size distribution and 5′ end nucleotide preference of siRNAs identified by deep sequencing. (A) NRDE-3-, (B) HRDE-1-, and (C) WAGO-1-bound small RNAs in indicated animals were deep sequenced. Size distribution and 5′ end nucleotide preference were analyzed.

Additional file 3: Figure S3.

CDE-1 interacts with SUSI-1(ceDIS3L2) in the germline. (A) → CDE-1::GFP was visualized by fluorescent microscopy at indicated developmental stages. White dashed lines show the borders of embryos or germlines at indicated developmental stages. Green dashed lines indicate P cell lineage at embryo stage. (B) → Western blotting analysis of CDE-1::GFP was performed after GFP immunoprecipitation. (C) → SUSI-1(ceDIS3L2) accumulated in the cytoplasm. Images of CDE-1::mCherry (largely colocalized with the P-granule, the upper panel) and GFP::SUSI-1 (in cytoplasm, the upper and lower panels) expression in the germline cells at young adult stage.

Additional file 4: Figure S4.

qRT-PCR analysis of susi-1 mRNA levels in indicated animals at the L3 stage. Data are presented as the mean ± SD (n = 3, biological replicates). *P < 0.05 (two-tailed Student’s t test).

Additional file 5: Table S1.

Strains used in this work.

Additional file 6: Table S2.

Primers used for quantitative real-time PCR analysis.

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit http://creativecommons.org/licenses/by/4.0/. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated in a credit line to the data.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Wang, Y., Weng, C., Chen, X. et al. CDE-1 suppresses the production of risiRNA by coupling polyuridylation and degradation of rRNA. BMC Biol 18, 115 (2020). https://doi.org/10.1186/s12915-020-00850-z

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI: https://doi.org/10.1186/s12915-020-00850-z

Keywords

  • rRNA
  • siRNA
  • Argonaute
  • risiRNA
  • CDE-1
  • SUSI-1
  • Uridylation
  • Inheritance

BMC Biology

ISSN: 1741-7007

Contact us