Dicer ribonucleases of plants and invertebrate animals including Caenorhabditis elegans recognize and process a viral RNA trigger into virus-derived small interfering RNAs (siRNAs) to guide specific viral immunity by Argonaute-dependent RNA interference (RNAi). C. elegans also encodes three Dicer-related helicase (drh) genes closely related to the RIG-I-like RNA helicase receptors which initiate broad-spectrum innate immunity against RNA viruses in mammals. Here we developed a transgenic C. elegans strain that expressed intense green fluorescence from a chromosomally integrated flock house virus replicon only after knockdown or knockout of a gene required for antiviral RNAi. Use of the reporter nematode strain in a feeding RNAi screen identified drh-1 as an essential component of the antiviral RNAi pathway. However, RNAi induced by either exogenous dsRNA or the viral replicon was enhanced in drh-2 mutant nematodes, whereas exogenous RNAi was essentially unaltered in drh-1 mutant nematodes, indicating that exogenous and antiviral RNAi pathways are genetically distinct. Genetic epistatic analysis shows that drh-1 acts downstream of virus sensing and viral siRNA biogenesis to mediate specific antiviral RNAi. Notably, we found that two members of the substantially expanded subfamily of Argonautes specific to C. elegans control parallel antiviral RNAi pathways. These findings demonstrate both conserved and unique strategies of C. elegans in antiviral defense.
The genome of Caenorhabditis elegans encodes three Dicer-related helicases (DRHs) highly homologous to the DExD/H box helicase domain found in two distinct families of virus sensors, Dicer ribonucleases and RIG-I-like helicases (RLRs). Dicer initiates the specific, RNAi-mediated viral immunity in plants, fungi and invertebrates by producing virus-derived small interfering RNAs (siRNAs). By contrast, mammalian RLRs trigger interferon production and broad-spectrum viral immunity, although one of the three RLRs may act as both a negative and positive regulator of viral immunity. In this study we developed a transgenic C. elegans strain for high-throughput genetic screens and identified 35 genes including drh-1 that are required for RNAi-mediated viral immunity. Genetic epistatic analyses demonstrate that drh-1 mediates RNAi immunity downstream of the production of viral siRNAs. Notably, we found that drh-2 functions as a negative regulator of the viral immunity. Thus, both nematode DRHs and mammalian RLRs participate in antiviral immune responses. Unlike mammalian RLRs, however, nematode DRH-1 employs an RNAi effector mechanism and is unlikely to be involved in direct virus sensing.
Citation: Lu R, Yigit E, Li W-X, Ding S-W (2009) An RIG-I-Like RNA Helicase Mediates Antiviral RNAi Downstream of Viral siRNA Biogenesis in Caenorhabditis elegans. PLoS Pathog 5(2): e1000286. doi:10.1371/journal.ppat.1000286
Editor: David S. Schneider, Stanford University, United States of America
Received: October 31, 2008; Accepted: January 5, 2009; Published: February 6, 2009
Copyright: © 2009 Lu et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This work was supported by a UCR Senate COR Research Fellowship and by NIH R01 AI0542447 (to S.-W.D.).
Competing interests: The authors have declared that no competing interests exist.
Innate immunity is active immediately upon pathogen attack and represents an ancient defense mechanism conserved in diverse multicellular organisms. Innate immunity is initiated by pattern recognition receptors (PRRs) that recognize conserved molecular patterns associated with microbes. Well-characterized PRR families include the transmembrane Toll-like receptors (TLRs) and the cytosolic NOD-like receptors (NLRs) and RIG-I-like RNA helicase receptors (RLRs), all of which contain members in vertebrates that recognize viral single- and/or double-stranded RNAs as the pathogen signatures 1–3. Recognition of pathogens by PRRs typically triggers protein-protein interactions of PRRs with downstream signaling factors leading to the nucleus translocation of a transcriptional factor such as NF-κB and the subsequent transcription of immunity effector genes. The Dicer family of ribonucleases also recognizes viral RNA like these PRRs to initiate the viral immunity in plants and invertebrates that is mechanistically related to RNA silencing or RNA interference (RNAi). Unlike TLR and RLRs, however, Dicer further processes the viral RNA trigger into small RNAs of 21–24 nucleotides to guide specific antiviral silencing .
In addition to two type III RNase domains and a dsRNA-binding domain (dsRBD), Dicer contains an RNA binding domain called PAZ and an N-terminal RNA helicase domain that is closely related to RLRs ,. The Dicer family proteins produce small interfering RNAs (siRNAs) and microRNAs (miRNAs) in many eukaryotes, which are loaded in an Argonaute (AGO)-containing effector complex to silence gene expression by RNA cleavage, translational arrest, or methylation of DNA and chromatin. In fungi, plants and Caenorhabditis elegans, siRNAs are further amplified in a process that depends on de novo synthesis of dsRNA by cellular RNA-dependent RNA polymerase (RDR).
Genetic requirements of the Dicer-initiated viral immunity have been characterized more extensively in Arabidopsis thaliana and Drosophila melanogaster using known mutants in various RNA silencing pathways . The prevailing model for antiviral silencing against RNA viruses is that it acts via the canonical dsRNA-siRNA pathway of RNAi. This is supported by the detection of virus-derived siRNAs (viRNAs) of two polarities covering the entire length of viral genomic RNAs in the infected cells and the identification of the siRNA-producing Dicers in the biogenesis of viRNAs in both D. melanogaster and A. thaliana , –. Almost all of the genes known to participate in A. thaliana antiviral silencing have been implicated in the RDR-dependent synthesis of dsRNA in transgene-induced RNA silencing , –. In D. melanogaster, antiviral silencing induced by distinct positive-strand RNA viruses including Flock house virus (FHV), requires the same set of the core components of the canonical RNAi pathway that are dispensable for the biogenesis and function of miRNAs ,,,. A recent study found that viral dsRNA produced during initiation of FHV progeny RNA synthesis is recognized by Dicer-2 (DCR-2) and diced into viRNAs to trigger antiviral silencing . Infection of mammalian cells with some DNA viruses induces production of virus-derived miRNAs capable of silencing the antisense mRNAs of the cognate viruses . However, there is currently no evidence for the production of viral siRNA in mammals in response to RNA viruses, suggesting that RNA viruses are sensed by unrelated PRRs in invertebrates and vertebrates .
C. elegans is an excellent model system for studying many aspects of biology, including host responses to bacterial pathogens ,. C. elegans lacks NLRs and NF-κB-like transcriptional factors but encodes a single TLR. C. elegans also encodes a family of Dicer-related helicases (DRH), DRH-1, DRH-2 and DRH-3, which are highly homologous to the DExD/H box RNA helicase domain found in Dicer and the mammalian RLR family composed of RIG-I, MDA5 and LGP2 ,,. The RNA silencing machinery of C. elegans is characterized by a single Dicer (dcr-1), 4 RDRs (eg, ego-1 and rrf1–rrf-3) and 27 AGOs ,. Both miRNAs and siRNAs are produced by DCR-1 whereas PIWI-interacting RNAs (piRNAs, also known 21U RNAs) is Dicer-independent. Processing both endogenous (endo) and exogenous (exo) dsRNA into siRNAs further requires the dsRNA-binding protein RDE-4 although distinct AGO and RDR proteins participate in endo and exo siRNA pathways , –. The C. elegans family of AGOs, the largest of any organisms examined to date, is divided into three subfamilies. The AGO and PIWI subfamilies are required for the biogenesis of miRNAs and piRNAs, respectively, but ergo-1 in the PIWI subfamily has an essential role in the production of endo-siRNAs , –. The third subfamily is worm-specific and contains 18 members, many of which such as rde-1, ppw-1, C04F12.1, sago-1, and csr-1, act in parallel or sequentially to mediate the exo-siRNA pathway –. The exo-siRNA pathway requires amplification by rrf-1 in the soma and ego-1 in the germline whereas rrf-3 is essential for the biogenesis of endo-siRNAs ,. Interestingly, exo-RNAi is enhanced in worm mutants defective for several components of the endo-siRNA pathway including eri-1, ergo-1 and rrf-3, suggesting antagonism between the two siRNA pathways ,,,,,.
A natural virus for C. elegans is not known. However, cultured primary cells and living animals of C. elegans can be infected respectively by Vesicular stomatitis virus (VSV) and Vaccinia virus and living animals support complete replication of the FHV RNA genome engineered to be transcribed from an integrated transgene –. Infection of VSV, which contains a negative-strand RNA genome, is associated with the production of VSV-specific small RNAs and is potentiated in both nematode cells derived from exoRNAi-defective C. elegans mutants (rde-1; rde-3, rde-4, and rrf-1) and wild-type cells depleted of either DCR-1 or C04F12.1, but is inhibited in rrf-3 and eri-1 mutants that exhibit an enhanced exoRNAi response ,. The positive-strand genome of FHV is divided into two RNAs. RNA1 (3.1 kb) encode the viral RNA-dependent RNA polymerase (RdRP) and can self-replicate independently of RNA2 (1.4 kb), which encodes the capsid protein. Although FHV is a natural insect virus, it replicates efficiently on outer mitochondria membranes of diverse eukaryotic cells, indicating conserved mitochondria targeting of the viral replication complex –. FHV RNA3 (387 nt) is a product of RNA1 replication and acts as mRNA of the B2 protein, a viral suppressor of RNAi (VSR) essential for FHV infection in D. melanogaster ,,,. We showed that replication of a B2-deficient FHV mutant occurred robustly in the rde-1 mutant nematodes but was severely inhibited in wild-type nematodes, indicating restriction of FHV replication by the exo-RNAi pathway in C. elegans . These studies together strongly indicate that C. elegans encodes an active antiviral RNAi pathway that is induced by either direct viral infection , or replication of a viral RNA genome initiated intracellularly , the latter of which bypasses the initial steps such as cell entry that occur in viral infection of natural hosts.
Here we describe development of a transgenic C. elegans strain for the genetic characterization of the antiviral RNAi pathway. Use of the reporter strain in a feeding RNAi screen led to the identification of a largest set of putative genes in antiviral RNAi pathway in any organism. In particular, we showed that drh-1 and drh-2 of the three nematode drh genes participated in the regulation of antiviral RNAi. An extensive genetic analysis indicated that unlike mammalian RLRs, C. elegans drh-1 acts downstream of virus sensing and viRNA biogenesis and that exogenous and antiviral RNAi pathways have distinct genetic requirements. Both the conserved and unique strategies of C. elegans in antiviral defense are discussed.
Identification of genes required for antiviral silencing in C. elegans by feeding RNAi
We have previously described a derivative of the infectious full-length cDNA clone of FHV RNA1, pFR1gfp , in which eGFP coding sequence replaces most of the VSR B2 coding sequence (Figure 1A). The inserted eGFP fused with the N-terminal 23 codons of B2, is expressed only from the recombinant RNA3 produced during replication of FR1gfp, but not directly from FR1gfp because its initiation codon is more than 2.7 kb away from the 5′-terminus of FR1gfp RNA (Figure 1A). FR1gfp is defective in RNAi suppression due to loss of B2 expression but not in replication so that productive FR1gfp replication and expression of eGFP from the FHV replicon occur only after antiviral RNAi is suppressed by either co-expression of B2 or genetic disruption of the antiviral RNAi pathway in cultured fruit fly and mosquito cells . To develop a model suitable for genetic screens to identify new components in antiviral RNAi, we generated C. elegans strains carrying a chromosomally integrated transgene that codes for FR1gfp under the control of a heat-inducible promoter.
(A) Genome structure and expression of wildtype FHV RNA1 (FR1) and its B2-deficient mutant, FR1gfp, that expresses the enhanced GFP in place of B2. (B) Detection of green fluorescence in FR1gfp reporter worms after feeding RNAi targeting specific genes or the commonly used L4440 vector as indicated, photographed 48 hours after induction of the replicon replication. (C) Accumulation of FR1gfp genomic (RNA1) and subgenomic RNA (RNA3) by northern blotting in FR1gf worms with (lanes 3–12) and without (lanes 1–2) feeding RNAi of specific worm genes. Two independent tests were analyzed for each E. coli strain. Methylene blue staining of total RNA was provided to show equal loading.
We found that no green fluorescence or only a tiny green spot in the pharynx area was observed in FR1gfp worms after heat induction of the FHV replicon transgene (Figure 1B, top left). In contrast, bright green fluorescence was detected throughout the animal body after FR1gfp worms were fed on the E. coli food that expresses rde-1 dsRNA, which depletes mRNA of rde-1 in a process referred as feeding RNAi (Figure 1B, top middle). Abundant expression of eGFP was also observed in FR1gfp worms after a loss-of-function rde-1 allele was introduced into FR1gfp worms by genetic crosses (data not shown). Northern blot hybridizations confirmed the abundant accumulation of the chimeric RNA1 and RNA3 in FR1gfp worms after rde-1 depletion, but FR1gfp replication was inhibited in FR1gfp worms without rde-1 depletion (Figure 1C, compare lanes 1/2 and 4/5). Productive replication of FR1gfp replicon was similarly rescued by the loss-of-function rde-1 allele in the second FR1gfp worm strain in which the FR1gfp transgene was integrated at a different chromosomal location (Figure 2B, and data not shown). Thus, as found previously in cultured fruit fly and mosquito cells , productive FR1gfp replication and detection of extensive eGFP expression in FR1gfp worms depend on the genetic disruption of the antiviral RNAi pathway, suggesting that FR1gfp worms could be screened for new components of the pathway by feeding RNAi.
(A) Accumulation of the FR1gfp replicon RNAs in genetic mutant worm strains carrying the same FR1gfp transgene array. Total RNA was also analyzed from wildtype N2 worms with (N2) and without the FR1gfp transgene (N2*) 48 hours after induction of the replicon replication (h.a.i.). (B) Induction of the RNAi immunity by the replicon in a worm integrant different from that analyzed in (A). (C) Molecular structures and genetic lesions of the drh-1 and drh-2 genes. (D) Accumulation of (-) viral siRNAs in single knockout worm mutants 48 hours after induction of the replicon replication. 45 µg of total small RNAs was loaded in each lane. A combination of 18 32P end-labeled DNA oligos corresponding to eGFP coding sequence in tandem was used as the probe for viral siRNA detection. The same filters were probed for miR-58 after stripping as the loading control. (E) Detection of drh-1 and drh-2 transcripts before and after induction of the replicon replication. Two independent tests were analyzed for each strain. (F) Time course analysis of the accumulation of the replicon RNAs in wildtype and mutant worms 2, 6, and 16 h.a.i. Total RNA extracted from FR1gfp rde-1 worms 48 h.a.i. was loaded as a control (lane rde-1*). Methylene blue staining of total RNA was provided to show equal loading.
To test this idea, we searched for antiviral RNAi factors among genes shown previously to play a role in exo-RNAi ,. The genes identified using the candidate gene approach include firstly dcr-1, rde-1, and rde-4, which, together with rrf-1 and C04F12.1, were shown previously to be required for antiviral RNAi against VSV and for exo-RNAi ,,,. A specific role of these genes in worm antiviral RNAi was verified by demonstrating genetic rescue of the B2-deficient FHV replicon in FR1gfp worms following introduction of genetic loss-of-function mutations in rde-1, rde-4, rrf-1 or C04F12.1 by genetic crosses (Figure 2A). These results showed that the B2-deficient FHV replicon transcribed from a nuclear transgene was silenced in FR1gfp worms by the same set of genes known to participate in worm antiviral immunity against VSV infection. Thus, the FR1gfp worm strain provided an alternative model to the VSV infection system for the genetic characterization of the RNAi-mediated antiviral immunity in C. elegans, including the use of FR1gfp worms for feeding RNAi screens.
In addition to dcr-1, rde-1, and rde-4, 32 of 98 candidate genes tested were required for silencing the viral replicon in C. elegans in three independent feeding RNAi screens (Figure 1B/1C, Table S1). Our result suggests that most of the RNAi factors identified from previous genetic and feeding RNAi screens, including mut-7 and mut-16 , may not contribute to antiviral RNAi. Nevertheless, our screen provided the largest set of putative antiviral RNAi factors in any organism (Table S1), which include rsd-2 (Figure 1B/1C), required for systemic RNAi , and drh-1. We focused on drh-1 identified from the feeding RNAi screen and its related gene drh-2 because of their homology to the mammalian RLR family of cytosolic sensors for RNA viruses ,,.
drh-1 is essential for worm antiviral RNAi that is negatively regulated by drh-2
drh-1 encodes one of the three closely related worm members of the RLR family ,. To verify the result from feeding RNAi, we identified presumptive null alleles of drh-1(tm1329) and drh-2(ok951) and introduced them respectively into FR1gfp worms by genetic crosses (Figure 2C). We did not examine drh-3 in this study because drh-3(tm1217) mutant worms are sterile . We found that drh-1 mutant worms exhibited no visible morphological and developmental phenotypes. However, drh-2 worms were noticeably smaller than wildtype worms at the same developmental stages and were late by ∼8 hours in laying eggs (data not shown), suggesting that drh-2 may have a role in development. Northern blot hybridizations detected mRNAs specific to drh-1 and drh-2 in wildtype worms and deletion of 483- and 789-nucleotide genomic DNA respectively in drh-1 and drh-2 mutants caused visible shifts of the corresponding mRNAs (Figure 2E). However, neither was transcriptionally induced 48 hours after the initiation of FR1gfp replication or earlier (Figure 2E and data not shown).
We found that RNAs 1 and 3 of the B2-deficient FHV replicon accumulated to high levels in drh-1 mutant worms as compared to wild-type N2 worms (Figure 2A, compare lanes 3/4 and 9/10). Thus, an essential role for drh-1 in antiviral silencing revealed by feeding RNAi experiments was confirmed by an independent approach. By comparison, the accumulation levels of the replicon RNAs 1 and 3 were similar in drh-1, rde-1 and rde-4 worms, but were higher in these worms than in rrf-1 and C04F12.1 mutant worms in at least five independent experiments (Figure 2A). These results indicate that antiviral silencing against the FHV replicon was inhibited in drh-1 worms as effectively as in rde-1 and rde-4 mutants, and more effectively than in rrf-1 and C04F12.1 mutants (Figure 2A).
In contrast, the FHV replicon was not rescued in drh-2 mutants (Figure 2A, lanes 11–12). Although longer exposure revealed low accumulation levels of the FHV replicon in wild-type worms, the accumulation of the FHV replicon was either undetectable or lower in drh-2 mutants than in wildtype worms (Figure 2A, compare lanes 17/18 and 21/22). Apparently this effect is not transgenic allele specific in that the same effect was also observed for another FR1gfp transgenic allele (Figure 2B, compare lane 28 and lane 25). As expected, fosmid WRW0640F2, which contains both drh-1 and drh-2 wild-type alleles, was able to rescue drh-1 and drh-2 function in the corresponding mutants when assayed for FR1gfp replication (data not shown). These results show that drh-1 is as important as rde-1 and rde-4 in the worm antiviral RNAi against FHV, whereas drh-2 may negatively regulate this immunity. Similarly reduced accumulation of the FHV replicon was also observed in worms defective for ergo-1 (Figure 2A, lanes 23 and 24), which encodes an AGO that is required for the biogenesis of endo-siRNAs but is antagonistic to exo-RNAi . Several lines of evidence indicate that drh-2 and ergo-1 act as negative regulators of antiviral RNAi rather than positive regulators of FHV replication. FR1gfp is defective in RNAi suppression but not in replication in fly and mosquito cells  and in worms because FR1gfp replicated to high levels in several single mutants including rde-4 (Figure 2A) and robust replication of FR1gfp was not inhibited by the drh-2 and ergo-1 alleles in rde-4;drh-2 (see the last section of Results below) and rde-4;ergo-1 (data not shown) double mutants. In addition, both drh-2 and ergo-1 negatively regulate exogenous RNAi (Figure 3, see below).
(A and B) unc-22 RNAi phenotype in response to unc-22 dsRNA microinjected at 25 and 100 µg/ml, respectively. 30 to 40 worms were used for unc-22 dsRNA injection. Shown here are the percentages of twitching and paralyzed F1 progenies of each injected worm collected between 8 and 32 hours post injection. The error bars indicate standard deviation for the paralysis phenotype. (C) Morphological phenotype of the F1 progenies of wildtype and mutant worms after feeding RNAi targeting dpy-13. All worm strains were synchronized before feeding RNAi.
We further performed time course analysis of the accumulation of the FHV replicon in wild-type and seven worm mutants 2, 6 and 16 hours after transcriptional induction of FR1gfp (Figure 2F). Primary transcripts of FR1gfp initially accumulated to comparable levels in wild-type and all of the seven mutant worm strains examined at two hours after heat induction, indicating that none of these mutant alleles had a major effect on the transcription of the FR1gfp locus . Six hours after induction, FHV RNA1 and its replication product RNA3 were detectable in rde-1, rde-4 and drh-1 mutants, but not in wild-type, rrf-1, C04F12.1, drh-2, or ergo-1 mutants. At 16 hours after induction, productive replication of the viral replicon also became visible in rrf-1 worms but not in C04F12.1, drh-2, or ergo-1 worms (Figure 2F). These data indicate that the viral RNA clearance was triggered by viral RNA replication in an RNAi-dependent process that might require early and simultaneous participation of DRH-1, RDE-1 and RDE-4.
Characterization of drh-1 and drh-2 mutants in response to exo-RNAi
DRH-1 was first identified as an interacting protein of DCR-1 and subsequent affinity purification coupled with mass spectrometry implicates all three DRH proteins as DCR-1 interactors ,. drh-3 mutant worms were defective in germline RNAi but were wild-type in somatic RNAi; however, both germline and somatic RNAi was dramatically reduced in worms treated with either drh-1 or drh-2 (or both) dsRNAs ,,,. While these data indicate that drh-3 is essential for germline RNAi, it was uncertain if a specific member of the DRH family plays an essential role in somatic RNAi since depletion of the homologous drh genes by dsRNA lacks specificity.
We found that drh-1 mutant worms, either with or without the FR1gfp transgene, remained as sensitive as wild-type worms to feeding RNAi targeting either the maternally expressed skn-1 (data not shown) or dpy-13 (Figure 3C), and to microinjection of dsRNA targeting muscle specific gene unc-22, which produces both the light (twitching) and severe (paralysis) knockdown phenotypes (Figure 3A/3B). Thus, drh-1 is dispensable for somatic RNAi, which is in contrast to its essential role in antiviral silencing. Nevertheless, we found a slightly lower percentage of the injected worms exhibiting paralysis in drh-1 worms than in wildtype worms (Figure 3A/3B), and the difference detected was statistically significant (P<0.05), illustrating that drh-1 worms exhibited a weak deficiency in somatic RNAi. These results suggest that DRH-1 may be more efficient to mediate RNAi in the soma of wild-type worms, but this function of DRH-1 is genetically redundant and could be substituted for by another DRH member in drh-1 mutant worms.
Surprisingly, drh-2 mutant worms exhibited enhanced sensitivity to the injection RNAi targeting unc-22 as compared to wild-type worms and the difference was more obvious when low concentration of dsRNA was injected (Figure 3A/3B). Feeding RNAi targeting dpy-13 led to mild dumpy phenotype in wild-type and drh-1 worms, but drh-2 worms displayed severe dumpy phenotype as did worm mutants known to exhibit an enhanced RNAi phenotype such as ergo-1 (Figure 3C) and eri-1 ,,. In contrast to wildtype and drh-1 worms, rde-1 worms were resistant to dpy-13 RNAi as expected (Figure 3C). These results indicate that somatic RNAi is partially suppressed by drh-2 in wild-type worms, which is similar to its inhibitory role in antiviral RNAi.
drh-1 and drh-2 are dispensable for the biogenesis of miRNAs, endo-siRNAs and piRNAs
drh-3 is required for the biogenesis of endo-siRNAs, but not for miRNAs or piRNAs ,. Production of endo-siRNAs is also dependent on ergo-1, which inhibits both somatic RNAi and antiviral silencing. To investigate the mechanism of drh-1 and drh-2, we further determined if either was involved in the biogenesis of the three classes of C. elegans small RNAs. We found that neither drh-1 nor drh-2 was required for the biogenesis of miRNAs (Figure 4A, lanes 5 and 6), which is also known to be independent of rde-4. Minor changes in the accumulation of miRNAs observed occasionally in drh-1 mutant worms were not reproducible (Figure 2D/3A/3B/5B). The rde-4-dependent endo-siRNAs K02E2.6 and X-cluster siRNAs also accumulated to wild-type levels in both drh-1 and drh-2 mutants (Figure 4A/4B). The recently characterized piRNAs also accumulated to wild-type levels in both drh-1 and drh-2 mutants as in rde-4, rde-1, rrf-1, ppw-2 and ergo-1 mutants (Figure 4B). Thus, drh-1 and drh-2 do not appear to contribute to the biogenesis of any of the known endogenous small RNAs in C. elegans, suggesting that drh-2 negatively regulates somatic RNAi and antiviral silencing in a mechanism distinct from ergo-1.
(A) Accumulation of K02E2.6 and X-cluster siRNAs as well as miR-58, miR-238, and let-7 and lin-4 miRNAs in wildtype and mutant worm strains with (lane 1) or without the FR1gfp transgene (lanes 2–9). 45 µg of total small RNAs was loaded in each lane. The same filter was repeatedly reprobed after stripping. Small RNAs loaded in lane 1 was extracted from FR1gfp worms 48 hours post induction. (B) Accumulation of 21U1 piRNA in wildtype and mutant worm strains in the absence of FR1gfp transgene. End-labeled DNA oligos complementary to endo-siRNAs, miRNA and 21U1 piRNA were used as the probes. Ethidium bromide staining of tRNAs was provided to show equal loading.
drh-1 acts downstream of rde-4-dependent production of viRNAs
An antiviral RNAi component may function in virus sensing, the biogenesis or the antiviral activity of viRNAs . FHV-specific viRNAs of the antigenomic polarity, (-)viRNAs, were detectable in both drh-1 and rde-1 mutants (Figure 2D, lanes 2 and 4). Probing for viRNAs of the genomic polarity resulted in a smear and no discrete bands were detected in any of the worm strains tested either before or after transcriptional induction of FR1gfp (data not shown). FHV viRNAs accumulated to much lower levels in worms than in fruit flies ,. ViRNAs in worm cells infected with VSV were only detected by the RNase protection assay , which is far more sensitive than Northern blot hybridization . We found that (-)viRNAs were undetectable in wild-type, drh-2 or ergo-1 mutant worms (Figure 2D, lanes 1 and 5; Figure 5B, lane 8), which is likely due to the inhibition of the viral replication (Figure 2A, lanes 3/4, 11/12, 23/24) and consequently lower levels of viral dsRNA for dicing in these worms. The FHV replicon replicated to similarly high levels in rde-1, rde-4 and drh-1 mutant worms (Figure 2A), but viRNAs were not detectable in rde-4 worms, unlike in rde-1 and drh-1 worms (Figure 2E). These results therefore show that RDE-4 is essential for the production of FHV viRNAs whereas either DRH-1 or RDE-1 is dispensable. However, since viRNAs produced in drh-1 and rde-1 worms were not able to inhibit the replication of the VSR-deficient viral replicon (Figure 2A), we further conclude that both RDE-1 and DRH-1 are required for the antiviral activity of viRNAs. The observations that the viral RNA trigger was detected and processed into viRNAs in rde-1and drh-1 mutant worms ruled out a direct role of either gene in virus sensing.
(A, C, E) Accumulation of the FR1gfp replicon RNAs in single and double knockout worm mutants 48 after replicon replication. (B) Accumulation of (-) viRNAs in single and double knockout worm mutants 48 after replicon replication as described in Figure 2. A combination of 18 32P end-labeled DNA oligos corresponding to eGFP coding sequence in tandem was used as the probe for viral siRNA detection. The same filters were probed for miR-238 after stripping. (D) unc-22 RNAi phenotype in response to unc-22 dsRNA microinjected at 100 µg/ml as described in Figure 3.
Characterization of antiviral silencing in double mutants
To determine the epistatic relationships among the identified antiviral RNAi components, we constructed seven double knockout worm mutants by genetic crosses. First, rescue of the VSR-deficient viral replicon was stronger in rde-1 worms than in the mutant worms defective for C04F12.1 (Figure 5C), which encodes an AGO closely related to rde-1 in the expanded group of AGOs specific to C. elegans. However, the viral replicon replicated to higher levels in the rde-1:C04F12.1 double mutant than in either single mutant (Figure 5C, compare lane 4 and lanes 2 and 3). Thus, there is an additive effect of the two mutant alleles in blocking antiviral RNAi, indicating parallel AGO pathways for antiviral silencing in C. elegans. Second, the viral replicon did not accumulate to higher levels in rde-4;drh-1 double mutant than in either rde-4 or drh-1 single mutant (Figure 5A, compare lane 6 and lanes 3 and 4). viRNAs were not detectable in rde-4;drh-1 worms (Figure 5B, lane 5), which was similar to rde-4 worms but distinct to drh-1 worms. These results illustrated that rde-4 and drh-1 act in the same antiviral RNAi pathway and placed rde-4 in the upstream of drh-1. Third, abundant viRNAs were detected in rde-1;drh-1 worms as was found in rde-1 and drh-1 single mutants, further confirming the above conclusion that neither gene is essential for viRNA production.
Fourth, we found that the viral replicon replicated to similar levels in rde-1, rde-4 single mutants and rde-1;drh-2 and rde-4;drh-2 double mutants (Figure 5A, compare lanes 11 and 12 with lanes 8 and 9). This result showed that the drh-2 mutant allele failed to enhance antiviral RNAi when either rde-4 or rde-1 was not functional, suggesting that the rde-4-initiated pathway was targeted by drh-2 for negative regulation. Fifth, the accumulation levels of the viral replicon were similar in the ergo-1;drh-1 double mutant and the drh-1 single mutant (Figure 5E), indicating that the ergo-1 mutant allele also became ineffective in enhancing antiviral RNAi when rde-4-initiated pathway was inactive. However, we found that the ergo-1;drh-1 double mutant exhibited enhanced sensitivity to somatic RNAi as did the ergo-1 single mutant (Figure 5D), further demonstrating that drh-1 was dispensable for exo-RNAi.
Recent studies demonstrate that viruses can infect, replicate, and assemble within C. elegans cells and that RNA viruses are targeted for silencing by the canonical RNAi pathway in C. elegans –. These findings suggest that C. elegans could become an important model for understanding basic aspects of virus–host interactions . In this work, we developed a C. elegans model for the genetic analysis of antiviral RNAi that exhibits several notable features. Our system is amenable to the powerful genetic tools in C. elegans since initiation of viral replication is inducible without the need for viral inoculation. The viral replication cycle in our system begins with translation of the viral RdRP in the cytosol from nuclear transcripts and bypasses the initial steps in virus entry during infection such as infection of worm cells by VSV. However, all of the five C. elegans genes known to participate in antiviral RNAi immunity against VSV infection were also required for inhibiting the replication of the FHV replicon. In addition, mutant alleles of genes in the endo-RNAi pathway that enhance exoRNAi response also increased potency of antiviral RNAi against both VSV (eri-1 and rrf-3) , and the FHV replicon (ergo-1). These data indicate that antiviral RNAi is triggered during intracellular viral RNA replication in the absence of receptor-mediated virus entry across the plasma membrane as is known for viral immunity initiated by mammalian RLRs. Furthermore, removal of VSR B2 enhances the sensitivity of the GFP-expressing FHV replicon to antiviral RNAi. This is in contrast to the use of VSR-expressing wild-type viruses in previous genetic analyses ,, which may explain why our pilot feeding RNAi screen led to the identification of a large set of putative antiviral RNAi factors.
Genetic requirements of antiviral RNAi in C. elegans
Our genetic analysis confirms earlier observations that antiviral RNAi in C. elegans overlaps the canonical dsRNA-siRNA pathway of RNAi –. For example, 35 known RNAi factors participate in the worm antiviral RNAi against FHV (Table S1). Antiviral RNAi against FHV is enhanced in both ergo-1 and drh-2 mutant worms that exhibit enhanced RNAi. Furthermore, this work together with previous studies shows that (i) antiviral RNAi induced by either FHV or VSV requires dcr-1, (ii) production of both VSV and FHV siRNAs was dependent on rde-4 and (iii) neither rde-1 nor drh-1 is essential for the biogenesis of viRNAs. These findings revealed a role of RDE-4, most likely with DCR-1 in a previously identified complex, in the sensing of viral RNA trigger and in the biogenesis of viRNAs. Whereas these data support a shared biogenesis pathway for viRNAs, exo- and endo-siRNAs in C. elegans , an indispensable role for rde-4 in the viRNA biogenesis is distinct from D. melanogaster in which DCR-2 but not the rde-4 homolog (R2D2), is essential for viRNA production .
Primary siRNAs processed directly from exogenous dsRNA are not sufficient abundant to detect by Northern blot hybridizations in rde-1 worms ,,, in contrast to FHV viRNAs. This difference is probably due to the robust supply of viral dsRNA from active viral RNA replication in rde-1 worms whereas the amount of exogenous dsRNA is limited in the absence of RDR-dependent dsRNA synthesis. Furthermore, our feeding RNAi screens indicate that a majority of the known exoRNAi factors may not participate in the worm antiviral RNAi against FHV (Table S1). In addition, whereas drh-1 is essential for antiviral RNAi against FHV, it is dispensable for exoRNAi. These data suggest that antiviral RNAi and exoRNAi pathways in C. elegans are genetically distinct even though both are initiated by RDE-4 and DCR-1.
An increased inhibition of the worm antiviral RNAi against FHV was observed in rde-1;C04F12.1 double mutant than in either single mutant, indicating that FHV is targeted by two parallel AGO-dependent antiviral RNAi pathways in C. elegans. This conclusion is also supported by previously observations that knockdown of either rde-1 or C04F12.1 individually enhances the VSV accumulation  and that RNAi suppression by B2 further increases FHV accumulation in rde-1 worms . Both RDE-1 and C04F12.1 belong to the substantially expanded subfamily of AGOs found only in worms and many members in this subfamily have been shown to act either in parallel or sequentially in exo-RNAi ,. Thus, expansion of this AGO subfamily in C. elegans may represent a unique strategy of host adaptation to viral infection, distinct or in addition to the strategy used by insects in which the evolution rate of antiviral RNAi factors DCR2 and AGO2 is much faster than that of their miRNA pathway counterparts DCR1 and AGO1 ,.
DRH-1 directs antiviral RNAi downstream of viRNA biogenesis
Several lines of evidence illustrate that drh-1 has a specific, non-redundant role in the rde-4-dependent antiviral RNAi pathway in C. elegans. Either depletion of drh-1 mRNA by feeding RNAi or a genetic lesion in drh-1 blocked antiviral RNAi against FR1gfp, an FHV-based replicon that does not express VSR B2 and thus exhibits a specific defect to suppress antiviral RNAi. B2 is a dsRNA/siRNA-binding protein which is located both inside the viral replication complex to inhibit the dicing of nascent dsRNA replicative intermediates into viRNAs and in the cytoplasm to inhibit the activity of viral siRNAs ,,,,. The antiviral RNAi against FHV was inhibited in drh-1 worms as efficiently as in rde-4 and rde-1 mutant worms. A time course analysis further suggests that DRH-1, RDE-4 and RDE-1 may all participate in the early induction of antiviral RNAi. Finally, epistatic analysis showed that the FHV replicon did not replicate to higher levels in rde-4:drh-1 double mutant than in either single mutant, demonstrating that drh-1 specifically acts in the rde-4-initiated antiviral RNAi pathway. Notably, inhibition of antiviral RNAi by the drh-1 mutant allele did not prevent the production of viRNAs in either drh-1 single mutant or rde-1:drh-1 double mutant worms, indicating that defects of drh-1 worms in antiviral RNAi were similar to rde-1 mutants but distinct to rde-4 worms. These data together show that drh-1 of C. elegans acts downstream of dcr-1 and rde-4 in the antiviral RNAi pathway and does not play a critical role in the sensing of the viral RNA trigger.
C. elegans DRHs may regulate specificity of distinct siRNA pathways
Previous knockdown experiments have established a genetic requirement for the DRH family of genes in the canonical RNAi ,. Use of drh-3 mutant worms has further shown that DRH-3 mediates germline RNAi and endo-RNAi, but is dispensable for somatic RNAi ,. Our results show that neither drh-1 nor drh-2 plays a role in the biogenesis of miRNAs, endo-siRNAs and piRNAs and that drh-1 mutant worms supported RNAi in the soma with only a negligibly reduced efficiency. Thus, drh-1 is essential for antiviral RNAi but is largely dispensable for both endo-RNAi and somatic RNAi. In contrast, drh-2 mutant worms exhibited enhanced response to both somatic RNAi and antiviral RNAi. Isolation of double drh knockout mutants, which is not possible to achieve by genetic crosses between the single mutants because of their close proximity, will be necessary to determine if the observed somatic RNAi in drh-1 worms is mediated by drh-3 and/or drh-2.
Current models indicate that DRH-1/2 and DRH-3 participate in the biogenesis of exo-and endo-siRNAs, respectively, in distinct complexes with DCR-1 and that primary siRNAs thus generated are loaded in a particular AGO to guide RDR-dependent amplification of secondary siRNAs required for specific degradation of target mRNA ,,,,. Results presented in this work indicate that DRH family proteins play an essential role in siRNA pathways by acting downstream of the DCR-1/RDE-4-dependent siRNA biogenesis to mediate both specific and redundant siRNA pathways. Since in vivo interactions of DRH proteins with DCR-1 and RDE-4 have been detected ,, we propose that DRH protein facilitate the binding of primary siRNAs to AGOs, the amplification of secondary siRNAs, or the targeting and cleavages of the mRNA. The essential role of DRH-3 and DRH-1 specifically in the endo-siRNA/germline exo-siRNA and viRNA pathways, respectively, may be due to tissue and cell-specific localization of DRH proteins and of dsRNA trigger and mRNA targets. In contrast, somatic RNAi may be mediated redundantly by DRH-1, possibly with DRH-3, which is supported indirectly by the observation that although all of the known endo-RNAi worm mutants are defective in the biogenesis of endo-siRNAs, enhancement of somatic RNAi were detected in rrf-3, eri-1 and ergo-1 mutants, but was not reported for drh-3 mutant worms. DRH-2 may compete with DRH-1 for binding to the same or a similar set of co-factors, thereby inhibiting DRH-1-dependent antiviral RNAi and somatic RNAi. This hypothesis is consistent with our observation that the drh-2 mutant allele failed to enhance antiviral RNAi against FHV in rde-1 and rde-4 mutant worms that are defective in the drh-1-dependent viRNA pathway.
Conserved antiviral function of RLR members in C. elegans and mammals
Our demonstration that the viral immunity is regulated by drh-1 and drh-2 in C. elegans indicates an evolutionarily conserved antiviral role of the RLR family between worms and mammals. In mammals, RLR members RIG-I and MDA5 are essential for controlling infection of two distinct sets of ssRNA viruses. Current models envision that recognition of specific viral RNA forms by the C-terminal repressor domain activates a signaling cascade via two caspase activation and recruitment domains (CARD) at the N-terminus that culminates in the transcription of cytokine genes and broad-spectrum immunity –. The third RLR member LGP2 is analogous to DRH-2 since it shares homology with RIG-I and MDA5 in the helicase and repressor domains without the N-terminal CARD domains, and appears to repress RIG-I signaling but contribute to MAD5 signaling –. Although the N-terminal regions of DRH-1 and DRH-3 are highly homologous, neither contains a CARD domain or is transcriptionally induced upon viral replication. Our genetic analysis further suggests that drh-1 directs antiviral RNAi downstream of both the sensing and the processing of the viral RNA trigger into viRNAs. This may explain why DRH proteins of C. elegans do not contain CARD domains, which mediate downstream signaling events by protein-protein interactions in mammals.
C. elegans genetics and culture
The Bristol strain N2 was used as the standard wild-type strain. Alleles used in this study are all derived from N2 and include rde-1(ne300), rde-4(ne337), drh-1(tm1329), drh-2(ok951), rrf-1(pk1417), ergo-1(tm1860), and C04F12.1(tm1637). The genotypes of rde-1 and rde-4 worms were confirmed using skn-1 feeding RNAi. The genotypes of the rest worm strains containing single or double mutations were confirmed by PCR and/or feeding RNAi targeting skn-1.
Transgene construct and transgenic worms
Transgene construct carrying FR1gfp replicon was a derivative of pFR1-3 by replacing the NcoI-SacI fragment of FHV RNA1 by the full length enhanced GFP coding region as described previously ,. This created a translational fusion of GFP with the N-terminal 23 amino acids of B2 and deletion of approximately 200 nucleotides from the B2 ORF. Animals were made transgenic by gonadal microinjection following standard protocol as described . Briefly, FR1gfp plasmid (final concentration 5 µg/µl) was mixed with the rol-6D plasmid pRF4 (final concentration 100 µg/µl) for injection into wild-type N2 animals. Generation of worm integrants carrying FR1gfp transgene and assay for viral replication was carried out as described previously .
Injection and feeding RNAi were carried out as previously reported. Briefly, for unc-22 dsRNA preparation, unc-22 single-stranded RNAs of both polarities were in vitro transcribed from a cDNA fragment amplified using T7 promoter-tagged primer unc22T7plus (TAATACGACTCACTATAGGAGTTGGGAGAGGATGAAGCT) and primer unc22T7minus (TAATACGACTCACTATAGGCCACCGTTGTCACGTGGAGGA). For injection RNAi, unc-22 dsRNA at 25 µg/ml or 100 µg/ml in water was delivered into intestine of young adult worms through microinjection. The injected worms were then transferred onto fresh NGM plates 8 hours post microinjection. Progenies produced between 8 and 32 hours post microinjection were scored for unc-22 phenotype. Feeding RNAi targeting skn-1 or dpy-13 was performed by feeding worms on E. coli. HT115 strains that express dsRNA corresponding to skn-1 and dpy-13, respectively. IPTG at final concentration of 1 mM was used for the induction of dsRNA expression. The P-value on the differences of unc-22 RNAi phenotype (paralysis) between worm strains was calculated using unpaired t test calculator (http://www.graphpad.com/quickcalcs/ttest1.cfm?FormatSD).
RNA preparation and Northern analysis
Total RNA was prepared using the TRI Reagent method (MRC, Inc.). Small RNAs were enriched using the mirVana kit (Ambion). For high molecular viral RNA analysis, 3 to 6 µg total RNA per lane was fractionated in 1.2% agarose gel. For small RNA analysis, 30 to 50 µg of enriched small RNAs per lane was resolved using 15% acrylamide denaturing gel along with chemically synthesized and end-labeled siRNAs as size markers. After electrophoreses, the RNA samples were transferred onto Hybond N+ membrane (Amersham Biosciences) and UV crosslinked using 1.8×105 µJ/CM2 as output power (SpectroLinker). For small RNA analysis, membranes were hybridized with 32P-labeled oligo DNA probes in PerfectHyb buffer (Sigma). For northern blot detection of drh-1 and drh-2 transcripts, 32P-labelled DNA probes were prepared using genomic DNA fragments amplified by PCR. Primer tm1329_internal_b (ATACTCTGCCTCGAGCCGAT) and primer Tm1329minus (TCAGTCGTATCTCCAATTTTCGA) were used to amplify genomic DNA as the drh-1 specific probe, while primer drh-21780plus (AGTAGCATTCGTTCGAGAGTT) and primer Ok951minus (TTGCTTTCCTGGACATGAAGTG) were used to generate the drh-2 specific probe. Sequences for oligo probes used for the detection of endogenous small RNAs were: miR-238, CTGAATGGCATCGGAGTACAAA; miR-58, ATTGCCGTACTGAACGATCTCA; miR-2, GCACATCAAAGCTGGCTGTGATA; lin-4, TCACACTTGAGGTCTCAGGGA; Let-7, AACTATACAACCTACTACCTCA; X-cluster siRNA, CGCGTATCTATTCAATTGAAT; K02E2.6 siRNA, ATCAGTTACTTGCCAATTTC; and 21U-1, CACGGTTAACGTACGTACCA
drh-1 and drh-2 functional rescue experiments
Transgenic lines in either drh-1(tm1329) or drh-2(ok951) background that carried an extrachromosomal array corresponding to WRW0640F2 were produced with microinjection, and were crossed respectively with drh-1(tm1329) and drh-2(ok951) animals homozygous for FR1gfp transgene. The F1 progenies in either drh-1(tm1329) or drh-2(ok951) background were then examined for GFP expression after being maintained at 20°C (drh-1) or 25°C (drh-2) for 36 hours after induction of the FR1gfp replicon replication. The complete loss or significant reduction of green fluorescence in F1 progenies that carried both FR1gfp and the WRW0640F2 extrachromosomal array, as compared to that in F1 animals that carried FR1gfp only, was considered as successful drh-1 function rescue. Likewise, increased GFP expression in F1 progenies that carried FR1gfp transgene only as compared to F1 progenies that carried both FR1gfp transgene and a WRW0640F2 extrachromosomal array, was considered as evidence for the restoration of drh-2 function.
GFP fluorescence images were collected using a CANON G2 digital camera mounted on an Olympus IMT-2 microscope.
Putative antiviral RNAi factors identified by feeding RNAi screens
(0.06 MB DOC)
We thank Craig Mello for providing the worm mutants used in this study and for hosting R.L. for part of this work in his lab, John Kim and Garry Ruvkun for the gift of 90 E. coli strains, and René Ketting and Ronald Plasterk for 8 E. coli strains for the feeding RNAi screen.
Conceived and designed the experiments: RL SWD. Performed the experiments: RL EY WXL. Analyzed the data: RL EY WXL SWD. Wrote the paper: RL SWD.
- 1. Ishii KJ, Koyama S, Nakagawa A, Coban C, Akira S (2008) Host innate immune receptors and beyond: making sense of microbial infections. Cell Host Microbe 3: 352–363.
- 2. Pichlmair A, Reis e Sousa C (2007) Innate recognition of viruses. Immunity 27: 370–383.
- 3. Yoneyama M, Fujita T (2008) Structural Mechanism of RNA Recognition by the RIG-I-like Receptors. Immunity 29: 178–181.
- 4. Ding SW, Voinnet O (2007) Antiviral immunity directed by small RNAs. Cell 130: 413–426.
- 5. Hammond SM (2005) Dicing and Slicing: The core machinery of the RNA interference pathway. FEBS Lett 579: 5822–5829.
- 6. Tabara H, Yigit E, Siomi H, Mello CC (2002) The dsRNA binding protein RDE-4 interacts with RDE-1, DCR-1, and a DExX-box helicase to direct RNAi in C-elegans. Cell 109: 861–871.
- 7. Aliyari R, Ding SW (2009) RNA-based viral immunity initiated by the Dicer family of host immune receptors. Immunol Rev 227: 176–188.
- 8. Bouche N, Lauressergues D, Gasciolli V, Vaucheret H (2006) An antagonistic function for Arabidopsis DCL2 in development and a new function for DCL4 in generating viral siRNAs. EMBO J 25: 3347–3356.
- 9. Deleris A, Gallego-Bartolome J, Bao J, Kasschau KD, Carrington JC, et al. (2006) Hierarchical Action and Inhibition of Plant Dicer-Like Proteins in Antiviral Defense. Science 313: 68–71.
- 10. Diaz-Pendon JA, Li F, Li WX, Ding SW (2007) Suppression of antiviral silencing by cucumber mosaic virus 2b protein in Arabidopsis is associated with drastically reduced accumulation of three classes of viral small interfering RNAs. Plant Cell 19: 2053–2063.
- 11. Fusaro AF, Matthew L, Smith NA, Curtin SJ, Dedic-Hagan J, et al. (2006) RNA interference-inducing hairpin RNAs in plants act through the viral defence pathway. EMBO Rep 7: 1168–1175.
- 12. Hamilton AJ, Baulcombe DC (1999) A species of small antisense RNA in posttranscriptional gene silencing in plants. Science 286: 950–952.
- 13. Li HW, Li WX, Ding SW (2002) Induction and suppression of RNA silencing by an animal virus. Science 296: 1319–1321.
- 14. Wang XH, Aliyari R, Li WX, Li HW, Kim K, et al. (2006) RNA interference directs innate immunity against viruses in adult Drosophila. Science 312: 452–454.
- 15. Boutet S, Vazquez F, Liu J, Beclin C, Fagard M, et al. (2003) Arabidopsis HEN1. A Genetic Link between Endogenous miRNA Controlling Development and siRNA Controlling Transgene Silencing and Virus Resistance. CurrBiol 13: 843–848.
- 16. Dalmay T, Hamilton A, Rudd S, Angell S, Baulcombe DC (2000) An RNA-dependent RNA polymerase gene in Arabidopsis is required for posttranscriptional gene silencing mediated by a transgene but not by a virus. Cell 101: 543–553.
- 17. Dalmay T, Horsefield R, Braunstein TH, Baulcombe DC (2001) SDE3 encodes an RNA helicase required for post-transcriptional gene silencing in Arabidopsis. EMBO J 20: 2069–2078.
- 18. Hernandez-Pinzon I, Yelina NE, Schwach F, Studholme DJ, Baulcombe D, et al. (2007) SDE5, the putative homologue of a human mRNA export factor, is required for transgene silencing and accumulation of trans-acting endogenous siRNA. Plant J 50: 140–148.
- 19. Morel JB, Godon C, Mourrain P, Beclin C, Boutet S, et al. (2002) Fertile hypomorphic ARGONAUTE (ago1) mutants impaired in post-transcriptional gene silencing and virus resistance. Plant Cell 14: 629–639.
- 20. Mourrain P, Beclin C, Elmayan T, Feuerbach F, Godon C, et al. (2000) Arabidopsis SGS2 and SGS3 genes are required for posttranscriptional gene silencing and natural virus resistance. Cell 101: 533–542.
- 21. Galiana-Arnoux D, Dostert C, Schneemann A, Hoffmann JA, Imler JL (2006) Essential function in vivo for Dicer-2 in host defense against RNA viruses in drosophila. Nat Immunol 7: 590–597.
- 22. van Rij RP, Saleh MC, Berry B, Foo C, Houk A, et al. (2006) The RNA silencing endonuclease Argonaute 2 mediates specific antiviral immunity in Drosophila melanogaster. Genes Dev 20: 2985–2995.
- 23. Aliyari R, Wu Q, Li HW, Wang XH, Li F, et al. (2008) Mechanism of induction and suppression of antiviral immunity directed by virus-derived small RNAs in Drosophila. Cell Host Microbe 4: 387–397.
- 24. Gottwein E, Cullen BR (2008) Viral and cellular microRNAs as determinants of viral pathogenesis and immunity. Cell Host Microbe 3: 375–387.
- 25. Kurz CL, Ewbank JJ (2007) Infection in a dish: high-throughput analyses of bacterial pathogenesis. Curr Opin Microbiol 10: 10–16.
- 26. Mahajan-Miklos S, Tan MW, Rahme LG, Ausubel FM (1999) Molecular mechanisms of bacterial virulence elucidated using a Pseudomonas aeruginosa-Caenorhabditis elegans pathogenesis model. Cell 96: 47–56.
- 27. Duchaine TF, Wohlschlegel JA, Kennedy S, Bei Y, Conte D Jr, et al. (2006) Functional proteomics reveals the biochemical niche of C. elegans DCR-1 in multiple small-RNA-mediated pathways. Cell 124: 343–354.
- 28. Tenor JL, Aballay A (2008) A conserved Toll-like receptor is required for Caenorhabditis elegans innate immunity. EMBO Rep 9: 103–109.
- 29. Fire A, Xu SQ, Montgomery MK, Kostas SA, Driver SE, et al. (1998) Potent and specific genetic interference by double-stranded RNA in Caenorhabditis elegans. Nature 391: 806–811.
- 30. Grishok A (2005) RNAi mechanisms in Caenorhabditis elegans. FEBS Lett 579: 5923–5939.
- 31. Grishok A, Pasquinelli AE, Conte D, Li N, Parrish S, et al. (2001) Genes and mechanisms related to RNA interference regulate expression of the small temporal RNAs that control C-elegans developmental timing. Cell 106: 23–34.
- 32. Hutvagner G, McLachlan J, Pasquinelli AE, Balint E, Tuschl T, et al. (2001) A cellular function for the RNA-interference enzyme Dicer in the maturation of the let-7 small temporal RNA. Science 293: 834–838.
- 33. Knight SW, Bass BL (2001) A role for the RNase III enzyme DCR-1 in RNA interference and germ line development in Caenorhabditis elegans. Science 293: 2269–2271.
- 34. Lee RC, Hammell CM, Ambros V (2006) Interacting endogenous and exogenous RNAi pathways in Caenorhabditis elegans. RNA 12: 589–597.
- 35. Parrish S, Fire A (2001) Distinct roles for RDE-1 and RDE-4 during RNA interference in Caenorhabditis elegans. RNA 7: 1397–1402.
- 36. Ruby JG, Jan C, Player C, Axtell MJ, Lee W, et al. (2006) Large-scale sequencing reveals 21U-RNAs and additional microRNAs and endogenous siRNAs in C. elegans. Cell 127: 1193–1207.
- 37. Batista PJ, Ruby JG, Claycomb JM, Chiang R, Fahlgren N, et al. (2008) PRG-1 and 21U-RNAs interact to form the piRNA complex required for fertility in C. elegans. Mol Cell 31: 67–78.
- 38. Das PP, Bagijn MP, Goldstein LD, Woolford JR, Lehrbach NJ, et al. (2008) Piwi and piRNAs act upstream of an endogenous siRNA pathway to suppress Tc3 transposon mobility in the Caenorhabditis elegans germline. Mol Cell 31: 79–90.
- 39. Tabara H, Sarkissian M, Kelly WG, Fleenor J, Grishok A, et al. (1999) The rde-1 gene, RNA interference, and transposon silencing in C-elegans. Cell 99: 123–132.
- 40. Tijsterman M, Okihara KL, Thijssen K, Plasterk RHA (2002) PPW-1, a PAZ/PIWI protein required for efficient germline RNAi, is defective in a natural isolate of C-elegans. Current Biology 12: 1535–1540.
- 41. Yigit E, Batista PJ, Bei Y, Pang KM, Chen CC, et al. (2006) Analysis of the C. elegans Argonaute family reveals that distinct Argonautes act sequentially during RNAi. Cell 127: 747–757.
- 42. Aoki K, Moriguchi H, Yoshioka T, Okawa K, Tabara H (2007) In vitro analyses of the production and activity of secondary small interfering RNAs in C. elegans. Embo J 26: 5007–5019.
- 43. Sijen T, Fleenor J, Simmer F, Thijssen KL, Parrish S, et al. (2001) On the role of RNA amplification in dsRNA-triggered gene silencing. Cell 107: 465–476.
- 44. Simmer F, Tijsterman M, Parrish S, Koushika SP, Nonet ML, et al. (2002) Loss of the putative RNA-directed RNA polymerase RRF-3 makes C. elegans hypersensitive to RNAi. Current Biology 12: 1317–1319.
- 45. Kennedy S, Wang D, Ruvkun G (2004) A conserved siRNA-degrading RNase negatively regulates RNA interference in C. elegans. Nature 427: 645–649.
- 46. Lu R, Maduro M, Li F, Li HW, Broitman-Maduro G, et al. (2005) Animal virus replication and RNAi-mediated antiviral silencing in Caenorhabditis elegans. Nature 436: 1040–1043.
- 47. Wilkins C, Dishongh R, Moore SC, Whitt MA, Chow M, et al. (2005) RNA interference is an antiviral defence mechanism in Caenorhabditis elegans. Nature 436: 1044–1047.
- 48. Schott DH, Cureton DK, Whelan SP, Hunter CP (2005) An antiviral role for the RNA interference machinery in Caenorhabditis elegans. Proc Natl Acad Sci U S A 102: 18420–18424.
- 49. Liu WH, Lin YL, Wang JP, Liou W, Hou RF, et al. (2006) Restriction of vaccinia virus replication by a ced-3 and ced-4-dependent pathway in Caenorhabditis elegans. Proc Natl Acad Sci U S A 103: 4174–4179.
- 50. Miller DJ, Ahlquist P (2002) Flock house virus RNA polymerase is a transmembrane protein with amino-terminal sequences sufficient for mitochondrial localization and membrane insertion. J Virol 76: 9856–9867.
- 51. Annamalai P, Rofail F, Demason DA, Rao AL (2008) Replication-coupled packaging mechanism in positive-strand RNA viruses: synchronized coexpression of functional multigenome RNA components of an animal and a plant virus in Nicotiana benthamiana cells by agroinfiltration. J Virol 82: 1484–1495.
- 52. Venter PA, Schneemann A (2008) Recent insights into the biology and biomedical applications of Flock House virus. Cell Mol Life Sci.
- 53. Li WX, Li H, Lu R, Li F, Dus M, et al. (2004) Interferon antagonist proteins of influenza and vaccinia viruses are suppressors of RNA silencing. Proc Natl Acad Sci U S A 101: 1350–1355.
- 54. Kim JK, Gabel HW, Kamath RS, Tewari M, Pasquinelli A, et al. (2005) Functional genomic analysis of RNA interference in C. elegans. Science 308: 1164–1167.
- 55. Sijen T, Plasterk RH (2003) Transposon silencing in the Caenorhabditis elegans germ line by natural RNAi. Nature 426: 310–314.
- 56. Tijsterman M, May RC, Simmer F, Okihara KL, Plasterk RH (2004) Genes required for systemic RNA interference in Caenorhabditis elegans. Curr Biol 14: 111–116.
- 57. Nakamura M, Ando R, Nakazawa T, Yudazono T, Tsutsumi N, et al. (2007) Dicer-related drh-3 gene functions in germ-line development by maintenance of chromosomal integrity in Caenorhabditis elegans. Genes Cells 12: 997–1010.
- 58. Sijen T, Steiner FA, Thijssen KL, Plasterk RH (2007) Secondary siRNAs result from unprimed RNA synthesis and form a distinct class. Science 315: 244–247.
- 59. Shaham S (2006) Worming into the cell: viral reproduction in Caenorhabditis elegans. Proc Natl Acad Sci U S A 103: 3955–3956.
- 60. Cherry S, Doukas T, Armknecht S, Whelan S, Wang H, et al. (2005) Genome-wide RNAi screen reveals a specific sensitivity of IRES-containing RNA viruses to host translation inhibition. Genes Dev 19: 445–452.
- 61. Obbard DJ, Jiggins FM, Halligan DL, Little TJ (2006) Natural selection drives extremely rapid evolution in antiviral RNAi genes. Curr Biol 16: 580–585.
- 62. Marques JT, Carthew RW (2007) A call to arms: coevolution of animal viruses and host innate immune responses. Trends Genet 23: 359–364.
- 63. Sullivan CS, Ganem D (2005) A virus-encoded inhibitor that blocks RNA interference in mammalian cells. J Virol 79: 7371–7379.
- 64. Chao JA, Lee JH, Chapados BR, Debler EW, Schneemann A, et al. (2005) Dual modes of RNA-silencing suppression by Flock House virus protein B2. Nat Struct Mol Biol 12: 952–957.
- 65. Pak J, Fire A (2007) Distinct populations of primary and secondary effectors during RNAi in C. elegans. Science 315: 241–244.