key: cord-0873953-1a5cy86i
authors: Xu, Jiuyue; Kong, Jing; Lyu, Bao; Wang, Xiaotong; Qian, Qi; Zhou, Xi; Qiu, Yang
title: The Capsid Protein of Rubella Virus Antagonizes RNA Interference in Mammalian Cells
date: 2021-01-21
journal: Viruses
DOI: 10.3390/v13020154
sha: 3e09db855adbe426465caabe62de059b32ff11d5
doc_id: 873953
cord_uid: 1a5cy86i

Rubella virus (RuV) is the infectious agent of a series of birth defect diseases termed congenital rubella syndrome, which is a major public health concern all around the world. RNA interference (RNAi) is a crucial antiviral defense mechanism in eukaryotes, and numerous viruses have been found to encode viral suppressors of RNAi (VSRs) to evade antiviral RNAi response. However, there is little knowledge about whether and how RuV antagonizes RNAi. In this study, we identified that the RuV capsid protein is a potent VSR that can efficiently suppress shRNA- and siRNA-induced RNAi in mammalian cells. Moreover, the VSR activity of the RuV capsid is dependent on its dimerization and double-stranded RNA (dsRNA)-binding activity. In addition, ectopic expression of the RuV capsid can effectively rescue the replication defect of a VSR-deficient virus or replicon, implying that the RuV capsid can act as a VSR in the context of viral infection. Together, our findings uncover that RuV encodes a VSR to evade antiviral RNAi response, which expands our understanding of RuV–host interaction and sheds light on the potential therapeutic target against RuV.

RNAi is known as a conserved gene silencing mechanism that evolved as an important antiviral immune defense mechanism in diverse eukaryotes. In the RNAi-mediated antiviral pathway, virus-derived dsRNA (vi-dsRNA) produced from viral infection and replication can be sensed by the type III endoribonuclease Dicer and then cleaved into small viral interfering RNA (vsiRNAs) 21-24 nucleotides (nt) in length [1] [2] [3] [4] [5] . These active vsiRNAs are integrated into the host Argonaute (Ago) protein to form the RNA-induced silencing complex (RISC) with the help of other host factors. Subsequently, RISC containing vsiRNAs directs the degradation of cognate viral RNAs by the endonucleolytic activity in a sequence-specific manner [6, 7] .

In response, many viruses encode VSRs to counteract the antiviral RNAi pathway [8, 9] . VSR proteins are widespread among RNA viruses that infect plants and animals and have also been identified in some DNA viruses [10] [11] [12] . In mammals, a number of mammalian virus-encoded VSRs, including Nodamura virus (NoV) B2 [13] [14] [15] [16] , influenza A virus (IAV) NS1 [17] , enterovirus 3A [18, 19] , and dengue virus (DENV) NS2A [20] have been demonstrated to act as bona fide VSRs to antagonize antiviral RNAi in the context of authentic viral infections. Furthermore, hepatitis C virus (HCV) core and NS2 [21] [22] [23] , human immunodeficiency virus (HIV) Tat [24] , Ebola virus VP35 [25, 26] , severe acute respiratory syndrome coronavirus N protein [27, 28] , the yellow fever virus (YFV) capsid [29] , and DENV NS4B [30] have been found to suppress the small hairpin RNA (shRNA)/siRNAmediated RNAi in vitro. The phenomena of numerous viruses encoding VSRs to suppress the RNAi pathway highlight the importance of antagonizing antiviral RNAi during viral life cycles.

RuV is a genetically simple, enveloped, positive-strand RNA virus belonging to the family Matonaviridae. RuV is the sole member of the genus Rubivirus [31] , while humans are the only natural hosts of RuV. Postnatal infections of RuV are usually mild, resulting in low-grade fever, scarlatiniform rash, or cervical lymphadenopathy [32] . However, maternal infection by RuV during pregnancy, particularly during the first trimester, can result in miscarriage and/or other congenital defects in newborns, collectively defined as congenital rubella syndrome (CRS) [33, 34] . CRS is typified by a characteristic pattern of birth defects that include cataracts, deafness, blindness, cardiac defects, and intellectual disability [35] . Up to now, the epidemics of RuV infection occasionally occur in developing countries and CRS remains a major public health concern all over the world [36] . To date, there are no approved antiviral therapies specific for RuV.

The RuV genome consists of a single positive-strand RNA of approximately 12 kb, which encodes two nonstructural proteins-p150 and p90-and three major structural proteins-E1, E2, and capsid. The RuV capsid protein is the sole virus-encoded protein component of the nucleocapsid that participates in many processes critical for the viral life cycle, including membrane association, RNA-binding [37, 38] , modulating viral RNA replication [39, 40] , mitochondrial rearrangements [41] , and inhibiting host protein translation by a nonenzymatic mechanism [42] . Our previous study demonstrated that the capsid protein encoded by the Semliki Forest virus (SFV), an important virus belonging to the Alphavirus genus in the family of Togaviridae, is a bona fide VSR that antagonizes antiviral RNAi in the context of SFV infection in cells [43] . Because the genomic structure and expression pattern of RuV and alphaviruses are similar, it would be intriguing to exploit whether the strategy of using capsid protein to suppress RNAi by SFV is also shared by RuV.

In this study, we identified that the RuV capsid could act as a potent VSR that inhibits Dicer-mediated siRNAs biogenesis by sequestrating dsRNAs and suppresses siRNAinduced RNAi. Moreover, we found that dimerization of the RuV capsid was required for its RNAi suppression activity. In addition, our data showed that the expression of the RuV capsid can rescue the replication of a VSR-defective model virus or replicon, implying that the RuV capsid can exert VSR function in a viral infection context.

For the reversal-of-silencing assay in mammals, the plasmid pEGFP-C1 was used to express the EGFP protein. For the expression of the RuV capsid and its derivatives in mammalian cells, their ORFs were cloned into vector pRK-Flag. To express proteins in Drosophila S2 cells, the ORFs were constructed into the insect expression vector pAc5.1/V5-HisB, respectively. The full-length cDNA of the FHV RNA1 and FHV RNA1 ∆B2 was described previously [12] . For the purification of the MBP fusion capsid protein, its ORF was inserted into the pFastBac-MBP vector [43] . The EGFP-siRNA (siEGFP) was chemically synthesized by Rui Bo, Guangzhou, China.

HEK293T and Vero cells were maintained in Dulbecco's modified Eagle medium (DMEM, Gibco) supplemented with 10% fetal bovine serum (FBS, Gibco, Grand Island, NY, USA), 100 U/mL penicillin, and 100 µg/mL streptomycin at 37 • C in an incubator with 5% CO 2 . The 293T-NoDice cell line was kindly provided by Bryan R. Cullen (Durham, NC, USA) and has been extensively used by us as previously described [18, 20, 43] . Drosophila S2 cells were cultured in Schneider insect medium (Gibco, Grand Island, NY, USA) with 10% FBS at 27 • C. Before transfection with FuGene HD reagent (Roche, Basel, Switzerland), the medium was changed to DMEM or Schneider insect medium containing 2% FBS without any antibiotic. 

The Ago2 CRISPR/Cas9 KO Plasmid (sc-400813, Santa Cruz Biotech, Santa Cruz, CA, USA) was used to knockout the ago2 gene in HEK293T cells according to the manufacturer's protocol. Briefly, after transfection with the CRISPR/Cas9 KO plasmids, HEK293T cells were cultured for 3 days and then selected by puromycin (1 µg/mL) (Invivogen, San Diego, CA, USA). The sorting of the RFP-positive single cells was performed on a BD FACSAria III (BD Biosciences, San Diego, CA, USA) upon excitation with a 554 nm wavelength solidstate laser. After reaching a sustainable size (>5 × 10 2 cells per clone), ∼10-200 cells of each clone were scraped off and collected using a 10 µL micropipette tip and screened for HDRmediated repair of the mutation. The resulting clones were confirmed by DNA-sequencing and Western blotting.

SFV (strain SFV4) and VSR-deficient SFV were from our laboratory; both were amplified in HEK293T cells [43] . EV-A71 (VR-1432, strain H) and VSR-deficient EV-A71 were from our laboratory; both were amplified in RD cells [18] . On the day of infection, the medium was changed with 2% FBS-DMEM, and then the viruses were added to HEK293T cells at an MOI of 1. Total RNAs were extracted at 12 and 24 h post infection (hpi) and subjected to qRT-PCR analysis.

For immunoprecipitation, transfected HEK-293T cells were harvested in IP lysis buffer (20 mM Tris, 100 mM NaCl, 0.05% n-Dodecyl β-D-maltoside (Sigma-Aldrich, St. Louis, MO, USA), and protease inhibitor cocktail (Roche, Basel, Switzerland)), followed by immunoprecipitation using M2 Flag antibody (Sigma-Aldrich, St. Louis, MO, USA) or mouse IgG (Proteintech, Rosemont, IL, USA) and protein-A/G agarose beads (Roche, Basel, Switzerland) according to the manufacturer's instructions. Briefly, cells were lysed at 4 • C for 30 min. Lysates were clarified at 12,000× g for 10 min at 4 • C and the lysates were precleared by incubation with protein-A/G agarose beads (Roche, Basel, Switzerland) at 4 • C for 2 h. Then, the pre-cleared lysates were incubated with antibodies (anti-Flag or anti-IgG) together with protein-A/G agarose beads (Roche, Basel, Switzerland) at 4 • C for 12 h. The antibody-bound complexes were washed five times with the same lysis buffer. Finally, proteins were extracted from the complexes and analyzed by Western blotting.

Cells were harvested in lysis buffer (50 mM Tris-HCl (pH 7.4), 150 mM NaCl, 1% NP-40, 0.25% deoxycholate, and a protease inhibitor cocktail (Roche, Basel, Switzerland)). The lysates were then subjected to 12% SDS-PAGE and Western blotting according to our standard procedures [18, 44] . The antibodies used in this study included anti-tubulin (1:3000), anti-His (1:10,000), anti-Flag (1:5000), and anti-Dicer (1:2000), which were purchased from Proteintech, Rosemont, IL, USA. The JAK1/JAK2 inhibitor Ruxolitinib (INCB018424) was purchased from Selleck, Houston, TX, USA (CAS No. 941678-49-5).

Total RNAs were extracted using TRIzol reagent (Takara, Tokyo, Japan) according to the manufacturer's instructions. For the detection of EGFP mRNA, 5 µg of total RNAs was subjected to denatured 1.5% agarose gels with 2.2 M formaldehyde. The separated RNAs were transferred onto the Hybond-A nylon membrane (GE Healthcare, Little Chalfont, Buckinghamshire, UK) and fixed at 120 • C for 15 min. The membranes were then hybridized with DIG-labeled probes in hybridization ovens at 65 • C overnight. The membranes were next incubated with anti-DIG antibody conjugated with alkaline phosphatase and exposed to a luminescent image analyzer LAS4000 (Fuji Film, Fuji, Japan). Probes for the detection of EGFP, Rp49, and GAPDH mRNA were complementary to nucleotide (nt) 520 to 700, nt 273 to 490, and nt 760 to 1060 of their ORF regions, respectively. The probe for the detection FHV RNA1 and subgenomic RNA3 was complementary to nt 2738 to 3058 of the B2 coding region. These probes were labeled with DIG-UTP (Roche, Basel, Switzerland) by in vitro transcription. For the detection of small RNAs, 20 µg of total RNAs was subjected to 7 M urea-15% PAGE and transferred to a Hybond-A nylon membrane (GE Healthcare, Little Chalfont, Buckinghamshire, UK). The membrane was chemically cross-linked in 1-ethly-3-(3-dimethylaminopropyl)-carbodiimide (EDC) at 60 • C. qRT-PCR using SYBR mix (Yeasen) [45] was carried out to detect the expression of EGFP mRNA, GAPDH mRNA, SFV NS1 mRNA, and EV-A71 mRNA.

RNA-IP was performed as previously described with minor modification [18] . Briefly, cells were lysed in a lysis buffer (20 mM Tris-HCl (pH 7.4), 200 mM NaCl, 2.5 mM MgCl 2 , 0.5% Triton X-100, 0.5 U/mL RNase inhibitor (Promega, Madison, WI, USA), and a protease inhibitor cocktail (Roche, Basel, Switzerland)) at 4 • C for 30 min. Lysates were clarified at 12,000× g for 10 min at 4 • C and the post nuclear lysates were pre-cleared by incubation with protein-A/G agarose beads (Roche, Basel, Switzerland) at 4 • C for 2 h. Then, the pre-cleared lysates were incubated with antibodies (anti-Flag or anti-IgG) together with protein-A/G agarose beads (Roche, Basel, Switzerland) at 4 • C for 12 h The antibodybound complexes were washed five times with the same lysis buffer. Finally, proteins or RNAs were extracted from the complexes and subjected to Western blot or Northern blot analysis, respectively.

The coding regions of the RuV capsid protein were cloned into pFastBac-MBP. Sf9 cells were infected with the recombinant baculoviruses and harvested at 3 days post infection. Cell pellets were re-suspended, lysed by sonication, and subject to centrifugation for 30 min at 11,000× g to remove debris. To get rid of the possible contaminant copurified from MBP-capsid via binding to RNA, the supernatant was treated with RNase A (Omega, Doraville, GA, USA) at a final concentration of 0.1 µg/µL for 4 h. All the purified proteins were concentrated using Amicon Ultra-30 filters (Millipore, Schwalbach, Germany). After that, the store buffer was exchanged to 50 mM 2-[4-(2-hydroxyethyl)-1piperazinyl] ethanesulfonic acid (HEPES)-KOH (pH 8.0). All proteins were quantified by the Bradford method and stored at −80 • C in aliquots. Proteins were separated on 10% SDS-PAGE and visualized by Coomassie blue.

A gel mobility shift assay was performed in 50 mM HEPES-KOH (pH 8.0), 100 mM NaCl, 2 mM MgCl 2 , 1 mM tRNA, 2 mM DTT, and 20 U RNasin, at a total volume of 10 µL reaction with the indicated amount of proteins and 0.1 pmol double-strand RNA (dsRNA) or single-strand RNA (ssRNA). The dsRNA was labeled with DIG-UTP (Roche, Basel, Switzerland) by in vitro transcription and derived from 1 to 200 nt of EGFP. Reactions were incubated for 30 min at 25 • C. The reactions were terminated by the addition of 2.5 µL 5× sample buffer (20 mM Tris-HCl (pH 8.0), 30% glycerol and 0.1% bromophenol blue). The nucleic acid-protein complexes were separated by electrophoresis on 1.5% agarose gels and transferred to the Hybond-A nylon membrane (GE Healthcare, Little Chalfont, Buckinghamshire, UK). After that, the membrane was subjected to cross-linking at 120 • C and was incubated with anti-DIG-alkaline phosphatase antibody (Roche, Basel, Switzerland), followed by incubating with CDP-STAR (Roche, Basel, Switzerland) for 15 min at 37 • C. The signals were then detected by X-ray film (Fujifilm, Tokyo, Japan).

To determine whether the RuV capsid protein acts as a VSR in vitro, we examined the capsid protein via a reversal-of-silencing assay as mentioned previously [18] . In this assay, HEK293T cells were co-transfected with the plasmids encoding EGFP and EGFP-specific shRNA (shEGFP), which is cleaved by Dicer to produce EGFP-specific siRNA and induces an RNAi response to degrade the EGFP transcript, together with a plasmid encoded Flagtagged RuV capsid or SFV capsid, as a positive control. After 48 h transfection, EGFP mRNA levels were determined by Northern blotting, and the capsid proteins of RuV and SFV were determined by Western blotting. As shown in Figure 1A , ectopic expression of the RuV capsid efficiently restored the expression level of RNAi-silenced EGFP mRNA, as well as the SFV capsid did, indicating that the RuV capsid contains the VSR activity. 

After identifying that the RuV capsid contains in vitro VSR activity, we sought to examine the mechanism of how RuV capsid antagonizes RNAi. The shRNA-induced RNAi pathway requires Dicer-mediated dsRNA cleavage into siRNA. To determine whether the RuV capsid blocks this step, small RNAs harvested from HEK293T cells were To investigate whether the VSR activity is dependent on protein expression levels, increasing amounts of RuV capsid were tested using the reversal-of-silencing assay ( Figure 1B) . The reversal effect of EGFP mRNA silencing increased progressively, along with the gradually increasing amounts of the transfected capsid-expressing plasmid ( Figure 1B) . We also detected EGFP mRNA at different time points, and the results showed that the reversal of EGFP mRNA silencing can be observed as early as 12 h after transfection of the capsid-expressing plasmid and was more effective at 24 and 48 h ( Figure 1C) .

To further confirm the VSR activity of the RuV capsid, we examined whether it can rescue the replication of a B2-deficient FHV RNA1 replicon (FHV-RNA1 ∆B2 ) in Drosophila S2 cells [12] . This mutant FHV RNA1 replicon lost the ability to suppress RNAi, leading to defective self-replication of FHV RNA1 and subgenomic RNA3 in S2 cells ( Figure 1D , compare lanes 1 and 2). Our data showed that the replication defect was partially rescued by the ectopic expression of either FHV B2 or the RuV capsid, respectively ( Figure 1D,  lanes 3 and 4) . Taken together, our findings indicate that the RuV capsid exhibits in vitro VSR activity in cells.

After identifying that the RuV capsid contains in vitro VSR activity, we sought to examine the mechanism of how RuV capsid antagonizes RNAi. The shRNA-induced RNAi pathway requires Dicer-mediated dsRNA cleavage into siRNA. To determine whether the RuV capsid blocks this step, small RNAs harvested from HEK293T cells were subjected to Northern blotting with DIG-labeled probes targeting EGFP siRNA. In the presence of the RuV capsid, a reduction in 22-nt Dicer-processed siRNA was detected (Figure 2A, lane 4) . Moreover, the production of 22-nt siRNA was gradually reduced along with the increasing protein expression levels of the RuV capsid ( Figure 2B,C) . This phenomenon was consistent with the EGFP mRNA levels observed in the reversal-of-silencing assays ( Figure 1A-C) .

In the RNAi pathway, when being processed from dsRNA, siRNAs are incorporated into RISC to mediate the cleavage of cognate RNAs [46] . Since we have found that the RuV capsid can inhibit shRNA-induced RNAi and Dicer-mediated siRNA production, it would be intriguing to examine whether the RuV capsid also suppressed siRNA-induced RNAi, which occurs after siRNA generation. To this end, Dicer-and AGO2-deficient HEK293T cells (NoDice and ago2 −/− cells) were co-transfected with the plasmids encoding EGFP and shEGFP or chemically synthesized EGFP-specific siRNA (siEGFP), together with the plasmid for the RuV capsid, respectively. As shown in Figure 2D ,E, the chemically synthesized siEGFP mediated the silencing of EGFP mRNA in NoDice rather than in ago2 −/− cells, confirming that siEGFP can be efficiently incorporated into RISC to direct the cleavage of cognate mRNAs. Our findings showed that ectopic expression of the RuV capsid efficiently restored the levels of siRNA-silenced EGFP mRNA in NoDice cells, indicating that the RuV capsid can suppress siRNA-induced RNAi in mammalian cells. EGFP and shEGFP or chemically synthesized EGFP-specific siRNA (siEGFP), together with the plasmid for the RuV capsid, respectively. As shown in Figure 2D ,E, the chemically synthesized siEGFP mediated the silencing of EGFP mRNA in NoDice rather than in ago2 −/− cells, confirming that siEGFP can be efficiently incorporated into RISC to direct the cleavage of cognate mRNAs. Our findings showed that ectopic expression of the RuV capsid efficiently restored the levels of siRNA-silenced EGFP mRNA in NoDice cells, indicating that the RuV capsid can suppress siRNA-induced RNAi in mammalian cells. 

To examine whether the RuV capsid inhibits siRNA production by directly binding to long dsRNA, we purified the recombinant maltose (MBP)-fusion capsid protein (MBPcapsid; Figure 3A , lane 3) and performed the electrophoretic mobility shift assay (EMSA) by incubating the in vitro-transcribed DIG-labeled 200-nt dsRNA together with the MBPcapsid. We found that the RuV capsid can directly interact with dsRNAs, and the shifting amount of labeled dsRNAs was increased along with the concentrations of MBP-capsid used in the reactions ( Figure 3B ). dsRNA in cells. For this purpose, we performed an RNA-IP assay in HEK293T cells ectopically expressing the Flag-tagged RuV capsid together with EGFP-specific dsRNA of 200nt in length. RNAs harvested from the Flag-precipitated complex were examined via Northern blotting with RNA probes that recognize positive-and negative-stranded EGFP sequences, respectively. We found that the RuV capsid indeed interacted with dsRNA (Figure 3C, lanes 5) . Together, we conclude that the RuV capsid can suppress RNAi by sequestrating dsRNA from Dicer cleavage. Subsequently, we sought to examine whether the RuV capsid can associate with dsRNA in cells. For this purpose, we performed an RNA-IP assay in HEK293T cells ectopically expressing the Flag-tagged RuV capsid together with EGFP-specific dsRNA of 200nt in length. RNAs harvested from the Flag-precipitated complex were examined via Northern blotting with RNA probes that recognize positive-and negative-stranded EGFP sequences, respectively. We found that the RuV capsid indeed interacted with dsRNA ( Figure 3C, lanes 5) . Together, we conclude that the RuV capsid can suppress RNAi by sequestrating dsRNA from Dicer cleavage.

After determining the in vitro VSR activity of the RuV capsid, we sought to identify the critical domains or amino acids required for its function. Previous studies show that the RuV capsid forms a disulfide-linked dimer [47] . Moreover, previous studies showed that homodimerization is critical for VSR's activity [18] [19] [20] 29, 43] ; we focused on the key region or residues responsible for the dimerization of the RuV capsid.

Each RuV capsid monomer consists of five antiparallel β-strands, including A-E, and a two-turn α-helix H between strands B and C ( Figure 4A ) [48] . To form a dimer, the residues of amino acids (aa) 169-175 of β-strand B from one monomer are hydrogen-bonded to the same but antiparallel β-strand B in the other monomer ( Figure 4A) . Moreover, the dimer can further form oligomerization through the interdimer molecular interface between Viruses 2021, 13, 154 9 of 14 capsid dimers, which involves β-strand C that is reported as the key residue essential for virus assembly and infection. In addition, Cysteine (C) at position 152 or 196 is reported to be important for the capsid's dimer [48] . Accordingly, we constructed a set of capsid protein mutants and truncations, and examined their activities to suppress RNAi via the reversal-of-silencing assay in HEK293T cells. Our data showed that the region of β-strands B, ranging from aa 169 to 175, is critical for the VSR activity of the capsid ( Figure 4B,  lane 7, ∆B) . The expression of capsid protein mutants and truncations was confirmed by Western blotting with anti-HA antibody ( Figure 4B ). On the other hand, either deleting the whole region of β-strand C or mutating the two key residues Glycine (G) to Prolines (P) within β-strand C showed no effect on the RNAi suppression activity of the RuV capsid ( Figure 4B, lanes 6 and 8, PVWP and ∆C) . The PVWP mutation was reported to disrupt the oligomerization of the RuV capsid but left its dimerization unaffected [48] . In addition, the C152A/C196A mutation did not affect the VSR activity ( Figure 4B, lane 9) .

To identify the critical residues within the region of aa 169 to 175 required for the VSR activity, we constructed several single-point or double-point mutations to alanine (A), and the resulting mutant capsid proteins were then examined via the reversal-of-silencing assay in HEK293T cells. The R169A, D171A, or R169A/D171A mutation (capsid R169A , capsid D171A , or capsid R169A/D171A ) significantly suppressed the activity of the RuV capsid to inhibit RNAi ( Figure 4C ) in HEK293T cells. In addition, we found that the replication defect of FR1-∆B2 cannot be rescued by the ectopic expression of either RuV capsid R169A/D171A or capsid ∆B ( Figure 1D , lanes 5 and 6). As well, the truncation mutations (∆B) abolished the dsRNA-binding activity of the RuV capsid examined by RNA-IP ( Figure 3C, lane 6) .

We sought to examine the relationship between the dimerization and the VSR activity of the RuV capsid. To this end, we performed co-IP assays with HEK293T cells ectopically expressing Flag-tagged capsid WT together with HA-tagged capsid mutants. As shown in Figure 4D , the protein-protein interactions between capsid WT and the mutant proteins (capsid R169A , capsid D171A , capsid K169A/D171A , and capsid ∆B ) were remarkably attenuated. Moreover, the self-interaction activity of capsid K169A/D171A or capsid ∆B was completely blocked ( Figure 4E ).

Together, our findings indicate that dimerization of the RuV capsid is required for the VSR activity, and R169 and D171 residues are critical for both activities.

We sought to further investigate the role of the RuV capsid as a VSR during viral infection in vertebrate hosts. Previous studies showed that in differentiated somatic cells, the VSR activity during viral infection should be examined in VSR-disabled mutant viruses, which trigger an effective RNAi response [18] . Since the infectious DNA clone of RuV was unavailable to us, we used other VSR-deficient viruses including SFV K124A/K128A and EV-A71 D23A instead in the subsequent tests. Our previous studies showed that the replication of these mutant viruses was restricted compared to that of wild type viruses due to loss of VSR activity, while either blocking the RNAi pathway or ectopic expressing the foreign VSRs can rescue the defective replication [18, 43] .

HEK293T or HEK293T-NoDice cells treated with Ruxolitinib, a JAK1 and JAK3 inhibitor to exclude the potential interference of the interferon I system, were infected with SFV WT or SFV K124A/K128A , and viral RNA accumulation was determined at 12 and 24 hpi, respectively. As expected, the viral RNA accumulation of SFV K124A/K128A was lower than that of SFV WT in HEK293T cells, while the genetic ablation of the RNAi pathway by Dicer knockout (NoDice) rescued the replication of SFV K124A/K128A ( Figure 5A ). The viral RNA replication of SFV K124A/K128A in HEK293T cells was increased by ectopic expression of RuV capsid WT or SFV capsid WT , but not the VSR-deficient mutants of the RuV capsid (capsid R1169A/D171A and capsid ∆B ) or SFV capsid (capsid K124A/K128A ) ( Figure 5A ). In addition, the viral RNA accumulation of SFV K124A/K128A in cells expressing the RuV capsid was comparable to that in NoDice cells, indicating that the rescuing effect of the RuV capsid on the replication a VSR-deficient virus is dependent of the RNAi pathway. (B) Vero cells were transfected with either empty plasmid or a plasmid-encoded SFV capsid WT , or capsid K124A/K128A as indicated. At 24 hpt, the cells were infected with EV-A71 WT or EV-A71 D23A at an MOI of 1. At 12 and 24 hpi, the levels of EV-A71 genomic RNAs in cells were determined by qRT-PCR. Cellular lysate was harvested and analyzed by Western blotting. Empty vector was used as a mock control. All data represent the means and standard deviations of three independent experiments. * p < 0.05 as measured by two-way ANOVA, in GraphPad Prism. n.s., not significant.

The VSR activity of the RuV capsid was further examined in Vero cells infected with EV-A71 WT or EV-A71 D23A . We found that the ectopic expression of RuV capsid WT , but not capsid R1169A/D171A and capsid ∆B , still enhanced the viral RNA replication of EV-A71 D23A ( Figure 5B ). Taken together, our findings indicate that the VSR activity of RuV capsid is sufficient to rescue the replication of VSR-deficient virus.

RuV is the etiological agent of a series of birth defects termed CRS that remains a global major public health concern, and better understanding of virus-host interactions would be helpful for identifying the pathogenesis of the viral disease and developing an antiviral therapy. RNAi is an antiviral response conserved in all eukaryotes, including mammals, and viruses encode VSRs to antagonize RNAi [49] . In this study, we found that the RuV-encoded structural protein capsid displayed VSR activity that suppresses Dicer-mediated siRNA production by sequestrating dsRNA and siRNA-induced RNAi in mammalian cells. Moreover, the VSR activity of the RuV capsid can rescue the defective replication of VSR-deficient viruses. Therefore, our findings support the notion that the RuV capsid can act as the VSR to facilitate viral replication by shielding viral dsRNA from Dicer cleavage and siRNA from RISC assembly.

Although belonging to different families, RuV and SFV share similar motif compositions, suggesting that their encoded proteins are likely to possess similar functions. Therefore, it is a rational prediction that the RuV capsid also contains VSR activity as does its counterpart, SFV. Moreover, our findings uncovered that the RuV capsid inhibits the RNAi pathway at two stages, including siRNA production and RISC assembly/function, which is consistent with the mode of action of the SFV capsid. Therefore, we speculate that using the capsid as VSR and targeting the steps of both siRNA production and RISC assembly/function are universal for multiple members in the family of Togaviridae to evade antiviral RNAi response.

Potent VSR activities were frequently observed in structural capsid proteins encoded by many viruses, such as the yellow fever virus capsid protein, SARS-CoV N, and SARS-CoV-2 N proteins. A virus-encoded capsid usually contains RNA-binding and dimerization activities, as association with viral genomic RNA, dimerization, and further oligomerization are necessary for viral nucleocapsid formation and the assembly of high-order structure of virions. In the case of RuV, our mutational analyses showed that mutation of R169A and D171A or deletion of the β-strand B region abolished the dimerization and dsRNA-binding of the RuV capsid, and, in turn, substantially reduced the VSR activity. Interestingly, the mutant PVWP, which was previously reported to disrupt the interaction between neighboring RuV capsid dimers to form high-order structure [48] , have no influence on the VSR activity of the RuV capsid. These data indicate that dimerization, but not oligomerization, is required for the VSR activity of the RuV capsid, which is in line with previous findings that dimerization is a common feature for many VSRs, including NoV B2, EV-A71 3A, and SARS-CoV-2 N.

In summary, our work demonstrates that the RuV capsid functions as a VSR in facilitating viral replication by preventing dsRNA from Dicer cleavage and RISC assembly/function in mammalian cells. The activity of VSR is dependent on the dimerization of capsid, which possibly provides a possible direction for future anti-RuV drug exploitation.

Moreover, it shows for the first time that RuV can antagonize antiviral RNAi, extending our knowledge about the interaction between Rubivirus and antiviral RNAi immunity.

Author Contributions: Conceptualization, Y.Q. and X.Z.; methodology, J.X.; software, J.X.; validation, J.K., B.L., X.W. and Q.Q.; formal analysis, J.X. and J.K.; investigation, J.X., J.K., B.L., X.W. and Q.Q.; resources, J.X.; data curation, J.X.; writing-original draft preparation, J.X.; writing-review and editing, Y.Q. and X.Z.; visualization, Y.Q. and X.Z.; supervision, Y.Q. and X.Z.; project administration, Y.Q. and X.Z.; funding acquisition, Y.Q. and X.Z. All authors have read and agreed to the published version of the manuscript. 

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The Nucleocapsid Protein of Coronaviruses Acts as a Viral Suppressor of RNA Silencing in Mammalian Cells

SARS-CoV-2-encoded nucleocapsid protein acts as a viral suppressor of RNA interference in cells

Yellow fever virus capsid protein is a potent suppressor of RNA silencing that binds double-stranded RNA

Role of RNA interference (RNAi) in dengue virus replication and identification of NS4B as an RNAi suppressor

Molecular biology of rubella virus

Rubella virus

Clinical and laboratory features of rubella

Teratogen update: Congenital rubella

Rubella and congenital rubella (German measles)

Rubella and congenital rubella syndrome: Global update

Phosphorylation of rubella virus capsid regulates its RNA binding activity and virus replication

Analyses of phosphorylation events in the rubella virus capsid protein: Role in early replication events

Localization of rubella virus core particles in vero cells

Novel replication complex architecture in rubella replicon-transfected cells

Rubella virus capsid associates with host cell protein p32 and localizes to mitochondria

Rubella virus capsid protein interacts with poly(a)-binding protein and inhibits translation

The Capsid Protein of Semliki Forest Virus Antagonizes RNA Interference in Mammalian Cells

Proteomics Profiling of Host Cell Response via Protein Expression and Phosphorylation upon Dengue Virus Infection

Feasibility Study of Mixing Throat Swab Samples for Severe Acute Respiratory Syndrome Coronavirus-2 Screening

RNA-based antiviral immunity

Oligomerization of the structural proteins of rubella virus

Rubella virus capsid protein structure and its role in virus assembly and infection

Small RNA-based antimicrobial immunity

We thank the core facility center of Wuhan Institute of Virology for technical help, and Kun Cai (Wuhan, China) for kindly providing materials.

The authors declare no conflict of interest.