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Severe acute respiratory syndrome coronavirus nsp1 protein suppresses host gene expression, including type I interferon production, by promoting host mRNA degradation and inhibiting host translation, in infected cells. We present evidence that nsp1 uses a novel, two-pronged strategy to inhibit host translation/gene expression. Nsp1 bound to the 40S ribosomal subunit and inactivated the translational activity of the 40S subunits. Furthermore, the nsp1-40S ribosome complex induced the modification of the 5'-region of capped mRNA template and rendered the template RNA translationally incompetent. Nsp1 also induced RNA cleavage in templates carrying the internal ribosome entry site (IRES) from encephalomyocarditis virus, but not in those carrying IRESs from hepatitis C and cricket paralysis viruses, demonstrating that the nsp1-induced RNA modification was template-dependent. We speculate that the mRNAs that underwent the nsp1-mediated modification are marked for rapid turnover by the host RNA degradation machinery.
Severe acute respiratory syndrome (SARS) coronavirus (SCoV), the causative agent of a newly emerged disease, SARS, is an enveloped virus that contains a single-stranded, positive-sense RNA genome of about 29.7 kb.1 Upon infection, the genome expression begins with the translation of gene 1, which constitutes the 5'-end two-thirds of the viral genome, to produce two large precursor polyproteins2,3 that are proteolytically processed by 2 virally encoded proteinases to generate 16 mature proteins, namely nsp1 to nsp162. While most of these gene 1 proteins are essential for viral RNA synthesis, some of them appear to have other biological functions.4–7
The most N-terminal gene 1 protein, nsp1, has unique biological functions; expressed SCoV nsp1 induces host mRNA degradation and suppresses host translation8. The expressed nsp1 suppresses the host antiviral signaling pathways as well9. Furthermore, nsp1 suppresses host gene expression, including type I interferon (IFN) production, by promoting host mRNA degradation and host translation suppression in infected cells10. The nsp1 of a closely related mouse hepatitis virus also suppresses host gene expression and is a viral virulence factor11. These data suggest that the SCoV nsp1-mediated suppression of host genes plays an important role in the pathogenesis of SARS. Accordingly, a delineation of the mechanisms of the nsp1-induced suppression of host gene expression is considerably important for gaining insight into SCoV pathogenesis at the molecular level. We designed the present study to uncover the mechanism of nsp1-induced suppression of host gene expression primarily by using an in vitro system. Our data revealed that nsp1 utilizes a novel, two-pronged strategy to inhibit host translation/gene expression.
We tested whether nsp1 protein could suppress translation in rabbit reticulocyte lysate (RRL). We expressed the full-length, wild-type nsp1 protein and its mutant form (nsp1-mt) carrying K164A and H165A mutations as glutathione S-transferase (GST)-tagged fusion proteins in E.coli followed by the removal of the GST tag to generate recombinant nsp1 and nsp1-mt proteins, respectively; nsp1-mt neither suppresses host translation nor promotes host mRNA degradation in expressing cells and infected cells10. After incubation of the nsp1 protein with RRL at 4°C for 30 min, we added different concentrations of capped and polyadenylated Renilla luciferase mRNA transcripts (rLuc RNA) to the mixture, and incubated the samples in the presence of [35S]methionine for 30 min. In control samples in which rLuc RNA was incubated with GST and nsp1-mt proteins, rLuc activity and labeled rLuc protein levels increased with rising mRNA concentrations. In contrast, the rLuc activity and labeled rLuc protein levels in the nsp1-containing sample was substantially lower than in the control samples; the rLuc activity and the radiolabeled rLuc protein levels in the presence of nsp1 were about 6–8% of the levels observed with GST or nsp1-mt (Fig. 1a and b), which clearly demonstrated that nsp1 efficiently inhibited the rLuc protein synthesis from capped rLuc RNA in RRL.
Next, we examined the effect of nsp1 on translation mediated by the internal ribosome entry sites (IRES) using in vitro-synthesized, bicistronic mRNAs, Ren-HCV-FF RNA and Ren-CrPV-FF RNA, in which expression of the upstream rLuc open reading frame (ORF) was mediated by cap-dependent translation and the translation of downstream firefly luciferase (fLuc) ORF was driven by hepatitis C virus (HCV) IRES and cricket paralysis virus (CrPV) IRES, respectively (Fig. 1c). Nsp1 efficiently suppressed the translation of capped fLuc RNA, m7G-FF, as well as translation driven by both IRESs (Fig. 1d–e). According to the current models of translation initiation, the CrPV-IRES recruits the 40S ribosomal subunit in the absence of any initiation factors12,13, which suggested to us that nsp1 could suppress the function of the 40S subunit or block translation at a post-initiation stage.
We tested whether nsp1 associates with the 40S ribosomal subunit and suppresses its function. We transfected 293 cells with mRNAs encoding nsp1, nsp1-mt or chloramphenicol acetyltransferase (CAT) proteins; all of these encoded proteins carried a C-terminal myc-His tag. At 8 h post transfection, we prepared the cell extracts and performed polysome profile analysis (Fig. 2a–2c). Expression of CAT and nsp1-mt showed similar polysome profiles, whereas nsp1 expression resulted in the accumulation of 80S monosomes, along with a significant reduction in the polysome abundance, in accordance with the observation that the expressed nsp1, but not nsp1-mt, suppresses host translation10. Western blot analysis of the resolved gradient fractions showed the co-sedimentation of the majority of nsp1, but not CAT and nsp1-mt, with the 40S ribosomal subunit (Fig. 2b). Likewise, only nsp1 co-sedimented with the 40S ribosomal subunit in RRL (Fig. 2d–2f). To confirm the interaction of nsp1 with the 40S ribosomal subunit, we transfected 293 cells with in vitro-synthesized mRNAs encoding nsp1-myc-His fusion protein, CAT-myc-His protein or nsp1-mt-myc-His protein and subjected the cell extracts to immunoprecipitation with anti-myc antibody. The immune complexes were washed with 0.5 M KCl, a stringent high-salt condition in which the 60S ribosomal subunits and the translation initiation factors are dissociated from the 40S subunits14. Consistent with our previous report10, the expression level of nsp1 was substantially lower than that of nsp1-mt or CAT. Nevertheless, an efficient co-immunoprecipitation of 18S rRNA and S6 ribosomal protein, core components of the 40S subunit, with nsp1, but not with CAT and nsp1-mt (Fig. 2g–2i), suggested the tight association of nsp1 with the 40S ribosomal subunit. Similarly, co-immunoprecipitation analysis showed that nsp1 also interacted with the 40S ribosomal subunit in RRL (Supplementary Fig. 1).
The finding that nsp1 inhibited CrPV-IRES-driven translation suggests that nsp1 could affect an event(s) downstream of the 43S complex formation that involves the binding of eIF2-GTP-Met-tRNA ternary complex and other initiation factors like eIF3 to the 40S subunit. To test the effect of nsp1 on 48S complex formation, in which the 43S complex binds to the mRNA, and 80S monosome assembly, we examined, by sucrose gradient fractionation, the levels of accumulation of these complexes on a radiolabeled mRNA template in the presence of nsp1. To analyze the effect of nsp1 on 80S formation, we incubated 32P-labeled rLuc RNA template with nsp1, GST, or nsp1-mt in RRL in the presence of cycloheximide (CHX). CHX treatment inhibits the elongation step, but does not affect 80S monosome assembly15. We used hippuristanol, which blocks eIF4A function and inhibits 48S complex formation, as a control16. CHX treatment induced 80S complex accumulation and hippuristanol inhibited it (Fig. 3a). Nsp1, but not GST and nsp1-mt, suppressed 80S complex formation (Fig. 3b). We tested the effect of nsp1 on 48S complex formation by incubating the samples with GMP-PNP and subsequently, subjecting them to sucrose gradient centrifugation; GMP-PNP does not affect 48S complex formation, whereas it blocks GTP hydrolysis by eIF2 in eIF2-GTP-Met-tRNA complexes and inhibits the release of eIF2 and subsequent joining of the 60S ribosomal subunit17. The 48S complex accumulated in the presence of GMP-PNP, but not in the presence of hippuristanol (Fig. 3c). Nsp1, nsp1-mt and GST did not suppress the 48S complex formation (Fig. 3d). These data showed that nsp1 did not inhibit 48S complex formation, but it suppressed 60S subunit joining.
Next, we performed a toeprinting analysis, which defines the positions of stalled ribosomes on the mRNA chain18. After initial incubation of RRL with nsp1, GST or nsp1-mt in the presence of CHX or a mixture of CHX and GMP-PNP, we added the rLuc RNA that had been pre-annealed with a 5'-end labeled primer to the samples. Subsequently, we subjected the samples to primer extension experiments without extracting the RNAs. In control groups, using GST and nsp1-mt, we detected a correctly positioned toeprint (TP-AUG), which was a premature primer extension termination signal that was induced by the presence of the stalled 40S subunit. The toeprint was approximately 15–17 nt downstream from the translation initiation codon in the presence of GMP-PNP and CHX, which allow 48S complex formation, but not 60S joining (Fig. 4a, lanes 5 to 7). In the presence of CHX, the control groups showed an additional band approximately 3 nt downstream from TP-AUG, which was most probably generated by the joining of the 60S subunits with the 40S complex positioned at the AUG (Fig. 4a, asterisk, lanes 2 to 4). Consistent with the observation that nsp1 suppressed the 80S complex formation (Fig. 3b), nsp1 caused a clear reduction in the amount of the toeprint for the 80S complex (Fig. 4a, lane 3). Compared to the observations in the control groups, the abundance of the TP-AUG was also reduced in the sample containing nsp1 (Fig. 4a, lanes 3 and 6), which suggested that nsp1 induced inefficient start-codon recognition. Unexpectedly, we detected several additional bands, both upstream and downstream of the TP-AUG, in the sample incubated with nsp1, but not in controls; a longer exposure of the CHX-treated sample clearly showed the same signals (data not shown). These data suggested that nsp1 induced the modification of rLuc RNA at several discrete sites, which blocked cDNA elongation on these modified RNAs.
We performed primer extension analysis to determine whether nsp1 indeed induced template RNA modification. After incubation of rLuc RNA with GST, nsp1 or nsp1-mt in RRL, as described above, we extracted the RNA and performed primer extension analysis using the same 5'-end labeled primer. In addition to the full-length primer extension product, only samples incubated with nsp1 showed several premature primer extension termination products, all of which corresponded to those detected in the toeprinting analysis performed in the presence of nsp1 (Fig. 4b). Northern blot analysis of rLuc RNA, extracted after incubation with nsp1 in RRL under the same conditions, did not show a significant reduction in the levels of full length rLuc RNA transcripts compared to the levels in the control groups (Supplementary Fig. 2). These data demonstrated that nsp1 induced the modification of capped rLuc RNA at several sites in the 5'-region without inducing extensive template RNA degradation.
To further characterize the nsp1-induced template RNA modification, we incubated cap-labeled rLuc RNA and 3'-end-labeled rLuc RNA, independently, with nsp1 in RRL in the presence of CHX and GMP-PNP; GST and nsp1-mt served as controls. After incubation, we analyzed the extracted RNAs on a 5% sequencing gel. The amounts of the intact cap-labeled rLuc RNA, which had been incubated with nsp1, were clearly lower than that of the controls (Figs. 5a and 5b), demonstrating that the 5'-end region of the capped rLuc RNA was removed in the presence of nsp1. Incubation of the 3'-end-labeled rLuc RNA with nsp1 resulted in the appearance of an additional band that migrated slightly faster than the intact RNA (Fig. 5a, asterisk). The total radioactivity of the intact 3'-end labeled rLuc RNA and the fast-migrating RNA band in nsp1-treated samples was similar to that of the intact 3'-end labeled rLuc RNA in the controls (Fig. 5b). To determine the approximate size of the fast-migrating band, we incubated 3'-end-labeled non-polyadenylated rLuc RNA with nsp1 in RRL; we used non-polyadenylated rLuc RNA because some of the polyadenylated rLuc RNA preparations had mRNA species with shorter poly(A) tails, which interfered with the positive identification of the truncated RNA products in the gel. We observed two major fast-migrating bands and their sizes were approximately 20 to 40 nt shorter than the full-length RNA template (Supplementary Fig. 3, asterisks). These data demonstrated that nsp1 induced the removal of the 5'-end, but not the 3'-end, from the rLuc RNA.
Next, we tested the translational competence of the rLuc RNA that had undergone the nsp1-induced modification. After incubation of the rLuc RNA in RRL in the presence of nsp1, GST or nsp1-mt, we added the same amount of CAT RNA to each sample as a spike RNA, extracted the RNAs and performed a second in vitro translation reaction without adding nsp1, GST or nsp1-mt. We performed this analysis to examine the translational competence of RNAs that were extracted from the first in vitro translation reaction. As expected, nsp1 suppressed the translation of rLuc RNA in the initial translation (Fig. 5c 1st, 5d). The rLuc RNA that had undergone the nsp1-mediated RNA modification was not efficiently translated into the rLuc protein (Fig. 5c 2nd, 5d), which demonstrated that the modified rLuc RNA was translationally inactive.
In addition to cap-dependent translation, nsp1 also suppressed translation mediated by IRESs derived from HCV and CrPV (Fig. 1). To address the question whether the nsp1-induced template RNA modification is specific for cap-dependent RNA template, we tested whether nsp1 induced the modification of IRES in RNA templates carrying HCV, CrPV and encephalomyocarditis virus (EMCV)-derived IRESs. We incubated the RNA transcripts, Ren-HCV-FF, Ren-CrPV-FF and Ren-EMCV-FF, a bicistronic RNA carrying EMCV IRES between the upstream rLuc ORF and the downstream fLuc ORF (Fig. 6a), in RRL in the presence of nsp1, GST or nsp1-mt. After incubation, we extracted the RNAs and subjected them to Northern blot analysis (Fig. 6). Nsp1 did not induce any RNA cleavage in Ren-HCV-FF and Ren-CrPV-FF (Fig. 6b and c, respectively). In contrast, nsp1 induced an RNA cleavage in Ren-EMCV-FF (Fig. 6d). A cleaved RNA fragment, detected by a probe that binds to the rLuc ORF, migrated similarly with the control RNA1, carrying the rLuc ORF and EMCV IRES (Fig. 6d), while the size of the other RNA fragment, detected by a probe that binds to fLuc ORF, was similar to the size of fLuc ORF in Ren-EMCV-FF. These data suggested that nsp1 induced the cleavage at or near the 3'-region of the EMCV IRES in Ren-EMCV-FF (Fig. 6d). These results demonstrated that nsp1 induced a template-dependent RNA cleavage in IRES-driven RNAs and that the nsp1-induced RNA modification was not specific for cap-dependent RNA template.
To assess the biological significance of nsp1 binding to 40S subunits, we examined whether nsp1 could modify the rLuc RNA without ribosomes. After pelleting down the ribosomes in RRL by centrifugation, we incubated the ribosome-free supernatant with the cap-labeled rLuc RNA and nsp1 in the presence of CHX and GMP-PNP; GST and nsp1-mt served as controls. Gel electrophoresis analysis of the extracted RNAs showed that the amounts of the cap-labeled rLuc RNA were similar among the three samples (Fig. 7a and 7b). To know whether the rLuc RNA that had been incubated with nsp1 in the absence of the ribosomes was translationally competent, we incubated the capped rLuc RNA with nsp1, GST, or nsp1-mt in the ribosome-free RRL. As expected, rLuc protein synthesis did not occur in the ribosome-free lysate (Fig. 7c, top panel). After incubation, we added the same amount of spike CAT RNA to the samples, extracted the RNAs and subjected them to in vitro translation reaction without adding nsp1, GST or nsp1-mt. The rLuc RNA that had been incubated with nsp1 in the ribosome-free RRL was translationally competent in the second in vitro translation assay (Fig. 7c, middle panel). These data suggested that the 40S subunit-bound nsp1 exerted the modification and inactivation of rLuc RNA.
We further tested whether the association of rLuc RNA with the 43S complex was required for nsp1-mediated template RNA modification by incubating the cap-labeled rLuc RNA with nsp1, GST or nsp1-mt in RRL in the presence of hippuristanol. Nsp1 did not affect the amount of the labeled RNA in the presence of hippuristanol (Fig. 7d), leading to our suggestion that the modification of the capped RNA required the association of template RNA with the nsp1-40S complex.
Nsp1 suppressed the translation mediated by CrPV IRES (Fig. 1) but did not induce the RNA cleavage in Ren-CrPV-FF (Fig. 6b). These data suggested that in addition to template RNA modification, the association of nsp1 with 40S ribosomal subunit also inactivated the translational function of 40S ribosomes. To further examine this possibility, we subjected Ren-CrPV-FF to in vitro translation in RRL in the presence of nsp1, GST or nsp1-mt. After incubation, we analyzed the aliquots of the samples by SDS-PAGE. As expected, nsp1, but not GST or nsp1-mt, suppressed both cap-dependent and IRES-dependent translation (Fig. 8a, 1st). We added the same amount of the spike CAT RNA to the remaining samples, extracted RNAs and performed a second in vitro translation analysis without adding nsp1, GST or nsp1-mt (Fig. 8a, 2nd, 8b). The cap-dependent rLuc gene translation, from Ren-CrPV-FF RNA that was exposed to nsp1 in the first in vitro translation reaction, was inhibited but the IRES-mediated fLuc translation was not inhibited. Thus, nsp1 suppressed CrPV IRES-mediated translation in the first in vitro translation reaction but did not induce the modification that inactivated the translational activity of CrPV IRES in the second in vitro translation assay. Like rLuc RNA (Fig. 5), incubation of cap-labeled Ren-CrPV-FF RNA with nsp1 resulted in the removal of the 5'-end region from this RNA (Fig. 8c). We interpreted these results to suggest that binding of nsp1 to 40S ribosomal subunits inactivated the translational functions of 40S ribosomes leading to the inhibition of CrPV IRES-driven translation in Ren-CrPV-FF. Collectively, these data showed that nsp1 suppressed translation by inactivating the translational functions of 40S ribosomal subunits and modifying the template RNA.
Host translational suppression that is often detected in virus-infected cells is an effective viral defensive strategy for suppressing host innate immune responses and freeing host translational machinery for viral-specific gene expression. Although many viral proteins that suppress host translation have been identified19–22, SCoV nsp18 and several herpes virus proteins23–26, including herpes simplex virus-1 vhs protein27, are known to promote destabilization of host mRNAs and suppress host translation. Vhs protein, which has a sequence similarity with known RNases, is indeed an RNase,28 induces RNA cleavage in RRL29, and degrades both host and viral mRNAs30. Unlike vhs, none of the known proteins share similarities with SCoV nsp1 in their sequence and structure. The biological activities of SCoV nsp1 also substantially differed from those of vhs, as nsp1 inactivated the translational functions of the 40S ribosomal subunit and modified RNA transcripts only in the context of its association with the 40S subunit. The strategy that SCoV nsp1 has evolved to bind to 40S subunits to exert its function appears to be an excellent one for blocking translation of both capped mRNAs and IRES-containing mRNAs, and for efficiently accessing host mRNAs, including those involved in host innate immune functions, and inactivating them.
By binding to the 40S ribosomal subunits (Fig. 2, Supplementary Fig. 1) and inactivating them (Fig. 8), SCoV nsp1 efficiently suppressed cap-dependent and IRES-mediated translation, including translation mediated by CrPV IRES. In contrast to SCoV nsp1, CrPV IRES-mediated translation is relatively insensitive to Drosophila Reaper, a a potent apoptotic inducer, which also inhibits translation by binding directly to the 40S subunit31.
Further studies are needed to determine how the binding of nsp1 to 40S ribosomal subunit inactivates their translational function. Using rLuc RNA as a template, we showed that the formation of the 80S complex, but not the 48S complex was inhibited in the presence of nsp1 (Fig. 3). Because the nsp1-40S complex also modified the 5'-region of the rLuc RNA (Figs. 4 and and5),5), it is possible that the nsp1-mediated RNA modification affected the formation of 48S and/or 80S complexes on these modified RNA templates (Fig. 3). We obtained somewhat conflicting results, which showed that nsp1 did not suppress the 48S assembly on rLuc RNA (Fig. 3d) but the 48S TP-AUG signal was reduced in the presence of nsp1 (Fig. 4a). These data may imply that some of the multiple toe-prints upstream of the TP-AUG, observed in nsp1-treated sample (Fig. 4a, lane 6), represent arrested 48S translation intermediates as a result of nsp1 inactivating the function of 40S ribosomal subunit leading to inefficient start site recognition; these arrested 48S translation intermediates could contribute to the signal observed for 48S complex formation (Fig. 3d). Furthermore, the nsp1-induced RNA modification alone cannot fully account for the substantially reduced luciferase protein synthesis from capped rLuc RNA (Fig. 1), highlighting the contribution of the translation inhibition function of nsp1 towards the suppression of reporter protein expression in RRL. To clarify the exact step in the translation of capped mRNAs that nsp1 inhibits, it would be useful to isolate an nsp1 mutant that retains the 40S subunit inactivating function but lacks the RNA modification function, and test the effect of this mutant on 48S and 80S complex formations.
In addition to the modification of the 5'-region of capped rLuc RNA (Fig. 5), Nsp1 also inactivated the translational competence of capped RNAs encoding CAT gene or fLuc gene (data not shown), suggesting that nsp1 could modify capped RNAs in general. Nsp1 induced a substantial reduction in the amount of full-length cap-labeled rLuc RNA (Fig. 5a), which suggested a possibility that the very 5'-end of the rLuc RNA, including the 7-methylguanosine cap and the radiolabeled phosphate group, was removed. Primer extension analysis of the rLuc RNA that had been incubated with nsp1 (Fig. 4b) revealed that nsp1 exerted the modification in several different regions at the 5'-end of rLuc RNA. An RNA signal that migrated slightly faster than the full-length rLuc RNA was detected after incubation of the 3'-end labeled rLuc RNA in the presence of nsp1 (Fig. 5a). Analysis of the nsp1-treated non-polyadenylated rLuc RNA further showed that the fast migrating species of rLuc RNA shown in Fig. 5a consisted of at least two bands that were roughly 20 to 40 nt shorter than the full-length rLuc RNA template (Supplementary Fig. 3). These data point to a possibility that the several premature primer extension termination products, which were obtained using nsp1-treated rLuc RNA (Fig. 4b), were derived from rLuc RNA species lacking different regions from their 5'-ends. Because nsp1 induced an internal RNA cleavage in Ren-EMCV-FF RNA (Fig. 6), we suspect that nsp1 also triggered a similar endonucleolytic RNA cleavage in the 5' region of rLuc RNA. We also noted that the amounts of the full-length primer extension product, obtained from rLuc RNA that had been incubated with nsp1, were not substantially different from the corresponding signal obtained from the control group (Fig. 4b). These data imply that nsp1 induced the removal of the entire or a portion of the cap structure without affecting the first 5'-end nucleotide from the full-length rLuc RNA. Probably, the putative nsp1-induced endonucleolytic cleavage and decapping activities both contributed to the translational inactivation of nsp1-treated rLuc RNA.
Nsp1 induced RNA cleavage in the EMCV IRES of Ren-EMCV-FF RNA but it did not induce the RNA cleavage in Ren-CrPV-FF and Ren-HCV-FF RNAs, revealing the template-dependent nature of nsp1-induced RNA cleavage. Furthermore, these data demonstrated that nsp1-induced RNA modification was not limited to cap-dependent RNA templates. Because the translation initiation factors, eIF4G and eIF4A, are required for cap-dependent and EMCV IRES-mediated translation but not for translation driven by the IRESs of HCV and CrPV32, these factors may be involved in the induction of nsp1-mediated endonucleolytic RNA cleavage of template RNAs. Alternatively, nsp1 may recognize a putative unique RNA element(s), which is present in EMCV IRES and is absent in HCV and CrPV IRESs, to induce the RNA cleavage in the EMCV IRES. Further studies using various RNAs carrying different types of IRESs will be necessary to distinguish between these two possibilities.
Two different mechanisms are conceivable as to how the nsp1-40S ribosome complex induces the RNA modification at the 5'-end region of capped rLuc RNA and at the EMCV IRES of Ren-EMCV-FF RNA. One is that the activated nsp1, induced by the binding of nsp1 to the 40S subunits, exerts the modification of these RNAs. Another possibility is that binding of nsp1 to the 40S subunits induces the activation or recruitment of a host factor(s) that modifies the template RNAs. It is also possible that some ribosome-associated factors are involved in nsp1-induced RNA modification. In fact, host endonucleases can destabilize host mRNAs during translational elongation in polysomes33,34. Because nsp1 modified the rLuc RNA during translation initiation (Figs. 3–5), the nsp1-mediated modification of the 5'-region of the capped RNA presents a novel strategy for modifying capped RNAs.
The expression of nsp1 in mammalian cells caused both host mRNA degradation and host translation inhibition8. Because host mRNAs that are not involved in active translation are delivered to host mRNA degradation pathways35, we hypothesize that host capped mRNAs that underwent the nsp1-mediated translation inhibition and modification in expressing cells and SCoV-infected cells are delivered to the host mRNA degradation machinery36 and efficiently degraded.
Efficient SCoV-specific gene expression occurs in infected cells, in which nsp1 suppressed host gene expression10, which implied that SCoV gene expression is somehow immune to the nsp1-induced suppression of gene expression in infected cells. Like many host mRNAs, coronavirus mRNAs are capped and polyadenylated37. Several mechanisms are conceivable for an apparent selective immunity of SCoV gene expression to the nsp1-induced translational suppression. One is that the SCoV-specific translation occurs in selected subcellular compartments, where the localization and the access of nsp1 is limited. Another possibility is that a viral or host-derived protein(s) selectively binds to SCoV mRNAs and facilitates SCoV-specific translation in the presence of nsp1. Alternatively, the efficient accumulation of SCoV mRNAs outcompetes the nsp1-induced translational suppression.
We cloned pST-fLuc by inserting the cDNA encoding the entire fLuc ORF region from the pGL3 control vector (Promega) into pSPT18 (Roche). We cloned the PCR-amplified full-length nsp1 and nsp1-mt genes into the pGEX vector (GE Healthcare), yielding pGEX-wt and pGEX-mt, respectively. We constructed pRL-EMCV-FL by replacing the fragment containing HCV IRES, fLuc gene and the 3'-noncoding region of pRC22F38 with that containing EMCV IRES, fLuc gene and the 3'-noncoding region of pT7-IRES-fLuc39.
We generated capped and polyadenylated CAT RNA, nsp1 RNA, nsp1-mt RNA, m7G-FF RNA, rLuc RNA, Ren-HCV-FF RNA, and Ren-CrPV-FF RNA by linearizing and transcribing the plasmids pcD-CAT, pcD-Nsp1-wt, pcD-Nsp1-mt10, pST-fluc, pRL-SV40 (Promega), pRC22F38, and pGL3/Ren/CrPV/FF40, respectively, using an mMESSAGE mMACHINE T7 Ultra kit (Ambion). We synthesized capped and non-polyadenylated Ren-EMCV-FF RNA from pRL-EMCV-FL after linearization by Cla I digestion at 288 nt upstream of the 3'-end of fLuc gene. We used TransIT mRNA (Mirus) for transfecting in vitro RNA transcripts into subconfluent 293 cells.
We purified GST-fused proteins expressed in E. coli BL21-CodonPlus DE3 cells (Stratagene) using glutathione Sepharose 4B affinity beads (GE Healthcare) followed by cleavage of GST from the GST-fused protein using PreScission protease (GE Healthcare).
We performed the translation reactions using Retic Lysate IVT™ Kit (Ambion). After preincubating RRL with nsp1, GST or nsp1-mt for 10 min at 4°C, we added RNA and incubated the samples at 30°C in the presence of [35S]methionine (1,000 Ci/mmol; MP Biomedicals). We resolved the translation products by 12% SDS-PAGE and visualized by autoradiography. We performed densitometric analysis using ImageJ software to quantify the bands. .
At 8 h post transfection of 293 cells with RNAs, we prepared the cell lysates using a buffer containing 50 mM Tris-HCl (pH 7.5), 5 mM MgCl2, 100 mM KCl, and 1% (v/v) Triton-X-100 and incubated the lysates with an anti-myc antibody (Upstate Biotech.) at 4°C. We collected the immune complexes after incubation with Protein G Plus-Agarose (Santa Cruz Biotech.) at 4°C followed by centrifugation. After washing the pellets three times in a buffer containing 10 mM HEPES (pH 7.4), 500 mM KCl, 2.5 mM MgCl2 and 1 mM DTT, we extracted RNA and performed Northern blot analysis using digoxigenin-labeled oligonucleotide probes41 to detect 18S and 28S rRNAs. We resolved the immunoprecipitated proteins in the pellets by SDS-PAGE and Western blot analysis.
At 8 h post transfection of 293 cells with RNAs, we prepared the cell lysates in a buffer containing 50 mM Tris-HCl (pH 7.5), 5 mM MgCl2, 100 mM KCl, 1% (v/v) Triton-X-100, 2 mM DTT, 100 μg ml−1 CHX, and 0.5 mg ml−1 heparin, applied them onto a 10% to 50% sucrose gradient containing the same buffer and centrifuged at 39,000 rpm in a Beckman SW41 rotor at 4°C for 2 h. After fractionating the gradient fractions using a gradient fractionator, we monitored the absorbance at 254 nm using an ISCO UA-6 spectrophotometer. We precipitated the proteins from each fraction using trichloroacetic acid and detected them by Western blot analysis. We extracted rRNAs from the fractions and visualized them on a gel by staining with ethidium bromide.
We performed the ribosome binding assay as described previously16. After preincubating RRL with GST, nsp-1, or nsp1-mt for 10 min at 4°C, we incubated the samples with [α-32P] UTP-labeled, in vitro transcribed rLuc RNA in the presence of 0.6 mM CHX or 1 mM GMP-PNP for 10 min at 30°C. After centrifugation through 10 to 40% sucrose gradients (38,000 rpm for 3.5 h in a Beckman SW41 rotor), we collected fractions from each gradient and determined the radioactivity in each fraction in a scintillation counter.
We performed toe printing analysis as described previously18,42. After pre-annealing the 5' 32P-labeled primer DNA (5'-TTT TTC TGA ATC ATA ATA ATT AA-3') (40,000 c.p.m.) to rLuc RNA by heating for 1 min at 65°C, followed by incubation at 37°C for 10 min, we preincubated RRL with 1 μg of GST, nsp1, or nsp1-mt for 10 min at 4°C and then incubated the samples with 0.6 mM CHX or 0.6 mM CHX and 1 mM GMP-PNP for 5 min at 30°C. After incubation, we added the primer-mRNA complexes to the samples and incubated for an additional 10 min at 30°C. We diluted the reactions 20-fold with buffer containing 0.5 mM CHX, 7 mM magnesium acetate, 100 mM potassium acetate, 0.5 mM dATP, dCTP, dGTP, and dTTP, 20 mM Tris-HCl (pH 7.4), 2 mM DTT, and 1 unit/μl SuperScript III (invitrogen) and incubated them at 30°C for 10 min. We resolved the extracted primer extension products on an 8% sequencing gel.
After preincubating RRL with GST, nsp-1, or nsp-1-mt for 10min at 4°C, we incubated the samples with 0.6 mM CHX or 0.6 mM CHX and 1 mM GMP-PNP for 5 min at 30°C. Then, we added rLuc RNA to the samples and incubated them for 10 min at 30°C. After extracting total RNAs, we incubated the RNAs with the 5'-end labeled primer as described above and performed primer extension using a Primer Extension System (Promega). We resolved the extracted primer extension products on 8% sequencing gel.
We generated the cap-labeled rLuc RNA by incubating uncapped rLuc RNA with vaccinia virus guanylyltransferase (Ambion) in the presence of [α-32P]GTP (3,000 Ci/mmol; MP Biomedicals) at 37°C for 1 h. We generated the 3'-end labeled rLuc RNA by incubating rLuc RNA with T4 RNA ligase (Ambion) in the presence of [32P]pCp (cytidine-3', 5' bis-phosphate; 3000 Ci/mmol, MP biomedicals) and ATP at 4°C for 16 h. We purified all labeled RNA transcripts with the RNeasy kit (Qiagen Inc.). We incubated the [32P]-labeled RNA transcripts with nsp1, GST or nsp1-mt in RRL. After 15 min incubation at 30°C in the presence of CHX and GMP-PNP, we extracted the RNAs and resolved them on 5% sequencing gel.
We thank Peter Sarnow (Stanford University, CA) for the pGL3/Ren/CrPV /FF plasmid, Stanley Lemon (University of Texas Medical Branch at Galveston) for the pRC22F plasmid and Jerry Pelletier (McGill University, Canada) and Junichi Tanaka (University of the Ryukyus, Japan) for hippuristanol. This work was supported by Public Health Service Grant AI72493. W.K. and C.H. were supported by the James W. McLaughlin Fellowship Fund.