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Journal of Virology, April 2006, p. 4157-4167, Vol. 80, No. 8
0022-538X/06/$08.00+0     doi:10.1128/JVI.80.8.4157-4167.2006
Copyright © 2006, American Society for Microbiology. All Rights Reserved.

Characterization of a Torovirus Main Proteinase

Saskia L. Smits,¹ Eric J. Snijder,² and Raoul J. de Groot^1*

Virology Division, Department of Infectious Diseases and Immunology, Faculty of Veterinary Medicine, Utrecht University, Utrecht, The Netherlands,¹ Molecular Virology Laboratory, Department of Medical Microbiology, Center of Infectious Diseases, Leiden University Medical Center, Leiden, The Netherlands²

Received 12 October 2005/ Accepted 2 February 2006

Top Abstract Introduction Materials and Methods Results Discussion References

 
Viruses of the order Nidovirales encode huge replicase polyproteins. These are processed primarily by the chymotrypsin-like main proteinases (M^pros). So far, M^pros have been studied only for corona-, arteri-, and roniviruses. Here, we report the characterization of the M^pro of toroviruses, the fourth main Nidovirus branch. Comparative sequence analysis of polyprotein 1a of equine torovirus (EToV) strain Berne, identified a serine proteinase domain, flanked by hydrophobic regions. Heterologous expression of this domain resulted in autoprocessing at flanking cleavage sites. N-terminal sequence analysis of cleavage products tentatively identified FxxQ(S, A) as the substrate consensus sequence. EToV M^pro combines several traits of its closest relatives. It has a predicted three-domain structure, with two catalytic ß-barrel domains and an additional C-terminal domain of unknown function. With respect to substrate specificity, the EToV M^pro resembles its coronavirus homologue in its preference for P1-Gln, but its substrate-binding subsite, S1, more closely resembles that of arteri- and ronivirus M^pros, which prefer P1-Glu. Surprisingly, in contrast to the M^pros of corona- and roniviruses, but like that of arterivirus, the torovirus M^pro uses serine instead of cysteine as its principal nucleophile. Under the premise that the M^pros of corona- and toroviruses are more closely related to each other than to those of arteri- and roniviruses, the transition from serine- to cysteine-based proteolytic catalysis (or vice versa) must have happened more than once in the course of nidovirus evolution. In this respect, it is of interest that a mutant EToV M^pro with a Ser¹⁶⁵Cys substitution retained partial enzymatic activity.

Top Abstract Introduction Materials and Methods Results Discussion References

 
Many positive-strand RNA viruses have adopted a "polyprotein" strategy to express (part of) their genome. Translation of viral RNA results in the synthesis of large multidomain protein precursors, which are proteolytically cleaved to yield a collection of intermediate and mature products. As a rule, polyproteins that are to yield secretory or membrane (glyco)proteins are processed by host-encoded proteinases within the lumen of the compartments of the exocytotic pathway (in particular the endoplasmic reticulum and the trans-Golgi network). Cytosolic processing, however, involves co- and posttranslational cleavage by viral proteinases that are present as distinct domains within the polyprotein itself (51, 72). Processing is often a prerequisite for the assembly of the viral RNA replicase/transcriptase. To add to the complexity, intermediate and mature products may have distinct functions in replication and may be required during different stages of the infection. Hence, the properties of the viral proteinases must be carefully tailored to ensure accurate and efficient cleavage in a substrate-specific and temporally well-coordinated fashion.

Many RNA virus proteinases resemble, in their mechanism of peptide hydrolysis and in their three-dimensional structure, either one of the prototypical cellular proteases papain and chymotrypsin. Papain and related proteinases are characterized by a two-domain +ß-fold with typically a cysteine and downstream histidine as the catalytic residues. Chymotrypsin has a distinctive two-ß-barrel structure in which the principal nucleophile, a serine residue, is part of a catalytic His-Asp-Ser triad (20, 49). Chymotrypsin-like serine proteinase domains have been identified within the polyproteins of among others flavi-, alpha-, luteo-, astro-, and sobemoviruses (13, 17, 29, 38, 42, 53, 66).Intriguingly, however, many viruses, for instance picorna-, como-, poty-, and caliciviruses, encode proteinases with a (predicted) chymotrypsin-like fold in which, instead of serine, a cysteine acts as the main catalytic residue (1, 5, 6, 27, 28, 31, 52, 55).

The order Nidovirales comprises a group of evolutionarily related enveloped (positive) stranded RNA viruses (corona-, toro-, arteri-, and roniviruses) (10, 15, 19, 26, 56, 58, 62), which have taken the polyprotein strategy to the extreme. The 5'-most two-thirds of the nidovirus genome is occupied by two large overlapping open reading frames (ORFs), ORF1a and ORF1b, the most downstream of which is only translated upon ribosomal frameshifting (9, 15, 18, 58). These ORFs specify two huge polyproteins, pp1a and the C-terminally extended frameshift protein pp1ab. In the case of the coronaviruses, pp1ab measures up to 7,200 amino acids in length, representing the largest polyprotein known to date. Among nidoviruses, the largest degree of sequence conservation is found within the ORF1b-encoded part of pp1ab, which contains the chief replicative domains (15, 19, 30, 57), i.e., the RNA dependent RNA polymerase (RdRp) and the helicase, as well as up to three additional domains, ExoN, NendoU, and 2'-O-methyltransferase (2'-O-MT), which display sequence identity to cellular RNA-modifying enzymes (8, 37, 57). Of the latter, the ExoN and 2'-O-MT domains are lacking in the arterivirus pp1ab.

Processing of the arteriviral and coronaviral polyproteins gives rise to 12 to 13 and 15 to 16 mature products, respectively, and an as yet unknown number of functional intermediates (57, 76). The N termini of the replicase polyproteins are processed by "accessory" papain-like proteinases (31). The vast majority of cleavages, however, are carried out by a single chymotrypsin-like main proteinase (M^pro), which is located in the C-terminal half of pp1a, flanked by hydrophobic regions that are thought to be involved in targeting the replicase to intracellular membranes (30, 54, 67, 71). Recent X-ray crystallographic analysis of the structures of corona- and arterivirus M^pros confirmed the predicted chymotrypsin-like two-ß-barrel fold (2, 4, 73). Interestingly, the corona- and arteriviral enzymes both possess an additional C-terminal domain, a feature not commonly seen in other viral and cellular chymotrypsin-like proteinases (2, 4). Also for the ronivirus M^pro, such an additional C-terminal domain was predicted (74).

One might surmise that the nidoviral M^pros, given their pivotal role in viral replication, are well conserved. Conversely, however, the primary sequences of the M^pros of corona-, roni-, and arteriviruses have diverged almost beyond recognition, and sequence identity is restricted to the regions immediately surrounding the main catalytic residues. Moreover, whereas the arteriviral M^pro is a serine proteinase with a canonical His-Asp-Ser catalytic triad (4, 64), the M^pros of the corona- and roniviruses are cysteine proteinases (28, 30, 43, 74). In the latter, the acidic catalytic residues have been lost and, apparently, these enzymes solely rely on the remaining catalytic His-Cys dyad (2, 73, 74).

Toroviruses have been poorly studied, but because of their relatively close phylogenetic relationship to coronaviruses they may in many respects represent "missing links" in comparative nidovirus studies. Here, we are the first to report the biochemical characterization of a torovirus M^pro. Upon analysis of the C-terminal half of pp1a of equine torovirus (EToV) strain Berne, we identified a chymotrypsin-like proteinase domain, which, like the M^pros of the arteri-, corona-, and roniviruses, is flanked by hydrophobic regions. When expressed in prokaryotic and mammalian cells, the proteinase domain autocatalytically released itself from its surrounding sequences. Surprisingly, the toroviral M^pro seems no more related to that of coronaviruses than to the M^pros of arteri- and roniviruses. Most saliently, in contrast to the M^pros of corona- and roniviruses, but like that of arteriviruses, the torovirus M^pro is a serine proteinase. A tentative processing scheme for the torovirus pp1a/pp1ab polyproteins is presented, and the implications of our findings for nidovirus evolution are discussed.

Top Abstract Introduction Materials and Methods Results Discussion References

 
Cells and virus. Equine dermis (Ederm) cells (American Type Tissue Culture Collection) and OST7-1 cells (23) were maintained as monolayers in Dulbecco's modified Eagle's medium (DMEM; BioWhitaker) supplemented with penicillin (100 IU/ml) and streptomycin (100 µg/ml) and 20% (DMEM20) or 10% (DMEM10) fetal calf serum, respectively. EToV strain Berne was propagated in Ederm cells as described previously (68). Recombinant vaccinia virus vTF7-3 (24) was obtained from B. Moss (NIH, Bethesda, MD).

Isolation of intracellular EToV RNA, cDNA synthesis, and PCR amplification. Total cytoplasmic RNA, isolated from the equivalent of 4 x 10⁶ EToV-infected Ederm cells (68), was subjected to reverse transcription-PCR (RT-PCR) with RNase H-free Moloney murine leukemia virus reverse transcriptase (Superscript II; Invitrogen) and with the Expand long template PCR system (Roche Diagnostics GmbH), according to the instructions of the manufacturers. Oligonucleotide primers 1071 and 1072 (Table 1) were designed after sequences located at the 5' end and 3' end of EToV ORF1A, respectively (59, 61). Primers 1288 and 1325 were designed after sequences from cDNA clones p133 and p135. These clones had been identified previously as EToV specific after screening of a genomic cDNA library (61) and had been tentatively mapped in ORF1a (E. J. Snijder, unpublished). Amplicons of approximately 5.5 kb were obtained, which were gel purified, blunt ended using large fragment DNA polymerase I (LFDP) according to the instructions of the manufacturer (Invitrogen), and cloned into an EcoRV-digested vector pWSK29 (70). Sequence analysis was performed commercially (BaseClear Labservices) using the ABI PRISM BigDye Terminators v3.0 cycle sequencing kit (Applied Biosystems) on at least two independent clones in both orientations.

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TABLE 1. Oligonucleotides used in this study for amplification or mutagenesis of EToV sequences

Preparation of EToV M^pro-specific antisera. The coding region for EToV M^pro amino acids (aa) 5 to 196 (as counted from the M^pro N terminus) was RT-PCR amplified with oligonucleotide primers 1548 and 1549 (Table 1). The resulting PCR product was digested with BamHI and EcoRV and inserted into HindIII (blunt ended)-BamHI-digested pQE9 (QIAGEN), yielding plasmid pQE-SS-M^pro(5-196). This expression vector, encoding a 22-kDa M^pro fragment fused at the N terminus to a His₆ tag, was introduced in Escherichia coli M15/pREP4 cells (QIAGEN). Expression of the recombinant protein was induced by adding IPTG (isopropyl-ß-D-thiogalactopyranoside) to a final concentration of 1 mM to bacterial cultures during exponential growth (optical density [OD] of 0.6). Bacteria were lysed 5 h after induction, and the His-tagged expression product was purified by Ni-nitrilotriacetic acid affinity chromatography using the XPRESS System version 2.0 (Invitrogen) according to the instructions of the manufacturer. The recombinant protein was eluted with a mixture of 20 mM sodium phosphate, 8 M urea, and 500 mM sodium chloride (pH 6.0) containing 500 mM imidazole. The eluate was concentrated on a Centricon concentrator (30-kDa cutoff; Amicon), dialyzed for 6 h against phosphate-buffered saline (PBS)-0.05% sodium dodecyl sulfate (SDS) and, finally, dialyzed for 16 h against PBS-0.02% SDS. New Zealand White rabbits were immunized subcutaneously with 100 µg of His-M^pro 1548/1549 fusion protein as described previously (12); the resulting antiserum was designated K158.

Antisera specific for the N terminus of EToV M^pro (K270), the C terminus of the M^pro (K272), or the N terminus of pp1a/pp1ab (K274) were prepared by repeated subcutaneous immunization of New Zealand White rabbits with 200 µg of the bovine serum albumin-coupled synthetic peptides NH₂-SVFSKATSPFTLHARPPK-COOH, NH₂-KPLQYFHVPSFWQPFKKQ-COOH, and NH₂-MFRILKNNTRETEQHLSSSK-COOH, respectively, as described previously (63).

Construction of prokaryotic and eukaryotic EToV M^pro expression vectors. For prokaryotic expression of EToV M^pro, residues 10376 to 11472 of the EToV genome were RT-PCR amplified with oligonucleotide primers 1606 and 1607 (Table 1). A product of the anticipated size of 1,112 bp was obtained, which was gel purified, inserted into plasmid pQE9, and cloned in E. coli M15/pREP4 cells (QIAGEN) as described above. The resulting expression vector, pQE-SS-M^pro, codes for a 42-kDa polypeptide, encompassing the EToV M^pro domain and flanking sequences.

The expression construct pQE9-SS-M^pro-GST is a pQE-SS M^pro derivative, which consists of nucleotides (nt) 10376 to 11473 of EToV ORF1a and nt 258 to 935 of the glutathione S-transferase (GST) gene from plasmid pGEX2T (Amersham Pharmacia Biotech). This expression cassette was produced via PCR with oligonucleotides 2124 and 2125 and conventional cloning procedures. It codes for a 60-kDa fusion protein consisting of the 366-amino-acid-residue M^pro domain with flanking sequences linked by a proline residue to amino acid residues 1 to 226 of the GST protein.

For mammalian expression, we employed the recombinant vaccinia virus-based vTF7-3 system. To generate a suitable expression vector, the 1606/1607 PCR amplicon, digested with BamHI and EcoRV, was cloned into SacI/BamHI-digested pBluescript K/S+ (Strategene) together with a double-stranded linker, consisting of oligonucleotides 1721 and 1722. The resulting plasmid, pBS-SS-M^pro, contains residues 10376 to 11472 of the EToV genome, placed under the control of the bacteriophage T7 promoter and provided in frame with an initiation codon in an optimal context for translation initiation (40).

Site-directed mutagenesis of (putative) active-site residues was performed by splicing overlap extension-PCR mutagenesis (35) and conventional cloning techniques; mutations introduced in M^pro and the primers used are listed in Table 1.

The dual-expression construct pBS-SS-M^pro-dual, is a pBS-SS-M^pro derivative in which, downstream of the M^pro sequences, a second expression cassette is inserted, which is placed under the translational control of the encephalomyocarditis virus (EMCV) internal ribosomal entry site (IRES; taken from plasmid pTN2) (69) and which consists of nt 821 to 1128 of EToV ORF1a fused in frame to nt 10.378 to 11.472 of the EToV genome (encoding M^pro and surrounding sequences) and nt 3 to 483 of the EToV N gene. This chimeric expression cassette was produced via a series of splicing overlap extension-PCRs with oligonucleotides 1638, 1640, 1902, and 1914 through 1918 (Table 1) and conventional cloning procedures. It codes for a 66-kDa fusion protein, consisting as listed from the N terminus to C terminus of (i) residues 1 to 103 of pp1a; (ii) the 65 aa residues immediately upstream of M^pro; (iii) the 292-residue M^pro domain; (iv) the 8 residues downstream of M^pro, including the cleavage site; and (v) residues 2 to 160 of the EToV N protein. In this fusion protein, the N-terminal M^pro cleavage site is abolished (QSAG) and the M^pro proteinase is inactivated by an active site Ser-to-Ala substitution.

Purification and N-terminal sequence analysis of M^pro cleavage products. EToV M^pro and M^pro-GST were expressed from plasmids pQE-SS-M^pro and pQE9-SS-M^pro-GST, respectively, in E. coli M15/pREP4 as described above. Of the 1-ml bacterial culture, the cells were collected by centrifugation at 14,000 rpm for 30 s, resuspended in 100 µl Laemmli sample buffer, and incubated for 5 min at 95°C. Proteins were separated in 15% SDS-polyacrylamide gel electrophoresis (PAGE) gels (20 µl cleared supernatant/lane), transferred to polyvinylidene difluoride membranes (Bio-Rad Laboratories), and subsequently stained with Coomassie brilliant blue R-250. The regions containing the cleavage products of interest were excised. N-terminal sequence analysis was performed by subjecting the proteins to 5 to 8 rounds of Edman degradation using standard procedures with a pulse-liquid protein sequencer (model 476A; Applied Biosystems).

Infection/transfection of mammalian cells and metabolic labeling. Monolayers of Ederm cells (1 x 10⁶ cells), grown in 35-mm wells, were washed once with PBS containing 50 µg/ml DEAE-dextran and then infected in PBS-DEAE with EToV at a multiplicity of infection of 5 PFU/cell. At 1 h postinfection (p.i.), the inoculum was replaced by 1 ml DMEM10 and incubation at 37°C continued.

Subconfluent monolayers of OST7-1 cells (2 x 10⁶ cells), grown in 35-mm wells, were infected with recombinant vaccinia virus vTF7-3 and, at 1 h p.i., transfected with 2 µg plasmid DNA as described previously (46).

Prior to metabolic labeling, the cells were depleted for methionine and cysteine for 30 min by replacing the tissue culture supernatant with 600 µl of prewarmed starvation medium (DMEM without L-cysteine and L-methionine [Invitrogen] supplemented with 5% FCS, 10 mM hydroxyethylpiperazine-N'-2-ethanesulfonic acid [HEPES; pH 7.4], 1 mM Glutamax). Then 100 µCi of Tran³⁵S-label (ICN) was added and the cells were labeled for the indicated length of time at 37°C.

After labeling, the cells were washed once with ice-cold PBS and then lysed on ice in 600 µl ice-cold lysis buffer (20 mM Tris-HCl, pH 7.5, 1 mM EDTA, 100 mM NaCl, 1% Triton X-100, and 1 µg/ml aprotinin, leupeptin, and pepstatin A each). Nuclei and cell debris were pelleted by centrifugation for 5 min at 14,000 rpm and 4°C, and the supernatant was subjected to radioimmunoprecipitation assay (RIPA). To this end, the lysates were adjusted to 2% SDS, diluted 10 times with detergent solution (50 mM Tris-HCl, pH 8.0, 62.5 mM EDTA, 0.4% Na deoxycholate, 1% NP-40, and 1 µg/ml of aprotinin, leupeptin, and pepstatin A each). RIPA was performed in a final volume of 1 ml with 3 µl of antiserum K158, K270, K272, K274 (see below), or R-EToV N (14). The immune complexes were adsorbed to Pansorbin cells (Calbiochem) for 30 min at 4°C, collected by centrifugation for 1 min at 14,000 rpm, and washed three times with detergent solution containing 0.25% SDS. The pellets were then resuspended in 25 µl Laemmli sample buffer and heated for 5 min at 95°C. Proteins were separated in 15% SDS-PAGE gels, which were fixed for 30 min in 50% methanol-10% acetic acid and dried for 60 min at 80°C. Labeled proteins were visualized by fluorography using Kodak intensifying screens.

Top Abstract Introduction Materials and Methods Results Discussion References

 
Comparative sequence analysis of EToV M^pro. The EToV Berne ORF1a was sequenced completely (GenBank accession no. DQ310701) and encodes a product, pp1a, 4,569 amino acids long; a ribosomal frameshift at the pseudoknot at the 3' end of ORF1a (58) would produce a C-terminally extended product, pp1ab, of 6,857 amino acids. During the preparation of our article, Draker et al. (22) reported the completion of the sequence of the bovine torovirus (BToV) strain Breda genome. These authors identified a BToV pp1a domain with sequence similarity to the adenosine diphosphate-ribose 1"-phosphatase processing enzyme family (22), a homologue of which also occurs at a similar topological position in pp1a of coronaviruses, but not in those of roni -and arteriviruses (57). Moreover, two proteinase domains were found: a cysteine proteinase within the N-terminal half of pp1a and a more C-terminally located serine proteinase (22). The pp1a polyproteins of EToV and BToV share 65% sequence identity and the three domains described by Draker and colleagures (22) are conserved in pp1a of EToV. They were in fact identified independently using standard protein-protein and PSI and PHI BLAST searches of the NCBI database with EToV pp1a sequences as a query.

The EToV serine proteinase domain, comprising residues 3278 to 3430, displayed sequence similarity with the SpIB serine protease of Staphylococcus aureus and with the pp1a serine proteinase of turkey astrovirus. Similarity was particularly evident in the areas surrounding the predicted active-site residues, with His⁷⁵, Asp¹¹³, and Ser¹⁹³ of S. aureus SplB (50); GenBank accession no. AF271715) aligning with His³³⁰⁴, Glu³³⁴⁷, and Ser³⁴¹⁶ in the EToV sequence (Fig. 1A). The putative EToV proteinase domain resides within pp1a/pp1ab at a relative position similar to that of the M^pros of other nidoviruses and, likewise, is flanked by hydrophobic regions (HR-1 and -2; Fig. 2A). Based upon these observations and upon the fact that no other chymotrypsin-like proteinase motifs were evident in the EToV pp1a/pp1ab sequence, we postulated the identified domain to represent the toroviral M^pro.

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FIG. 1. Identification and sequence comparison of the toroviral Mpro. (A) Alignment of EToV strain Berne Mpro with SplB of Staphylococcus aureus. Standard and PHI and PSI BLAST searches with pp1a residues 2385 to 4570 as a query revealed sequence identity across an extensive region (residues 3278 to 3430) with serine proteinase SplB of Staphylococcus aureus. Active-site residues predicted for SplB and corresponding residues in the EToV sequence are boxed and indicated by #; predicted key residues of the S1 pocket are shown in bold and indicated by @. Residues of EToV Mpro are presented as numbered from the initiating Met1 of pp1a. (B) Multiple sequence alignment of corona-, arteri-, roni-, and torovirus Mpro domains. Clustal X-based alignments of coronavirus, arterivirus, and gill-associated okavirus (GAV) Mpros, generated previously (3, 4, 74), were used to align the EToV and BToV sequences. Abbreviations of virus names and GenBank accession numbers for the sequences are as follows: TGEV, porcine transmissible gastroenteritis virus (group 1; CAB91144); MHV, mouse hepatitis virus strain A59 (group 2; NC_001846); SARS, SARS coronavirus (group II; NC_004718); IBV, avian infectious bronchitis virus (group 3; AY692454); EToV, equine torovirus strain Berne; BToV, bovine torovirus strain Breda 1 (AY427798); GAV, gill-associated okavirus (AF227196); EAV, equine arteritis virus (NC_002532); LDV; lactate dehydrogenase-elevating virus neurovirulent type C (NC_02534); and PRRSV, porcine reproductive and respiratory syndrome virus strain Lelystad (AY588319). Residues shared by a torovirus Mpro and any of the other sequences are indicated by dark shading; residues conserved between Mpros of different nidoviruses are indicated by light shading. Residue numbers for the mature Mpros of arteri-, corona-, and roniviruses are given; residues of EToV Mpro are numbered from the initiating Met1 of pp1a. Residues of the catalytic center and the S1 specificity pocket are boxed. Squares indicate the catalytic His and Ser/Cys residues, as well as the catalytic Asp residues of arterivirus Mpros; the latter are aligned with SARS coronavirus and TGEV residues, which in the tertiary structure of the coronavirus Mpro occupy an equivalent main chain position. Triangles indicate key residues involved in P1 substrate binding.

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FIG. 2. Autocatalytic processing of torovirus Mpro in E. coli. (A) Schematic representation of the EToV polymerase polyprotein pp1ab with the ORF1a- and ORF1b-encoded polypeptides shown as boxes (top). Also shown is the domain organization of the C-terminal half of pp1a with hydrophobic regions depicted as gray boxes. The Mpro domain and flanking hydrophilic sequences (indicated as a white box) were cloned in pQE9 and placed under the control of an IPTG-inducible bacteriophage T5 promoter (indicated by the black box and arrow). Furthermore, the structure of a construct encoding Mpro fused to GST is shown. White arrowheads indicate (predicted) Mpro cleavage sites (bottom). (B) Prokaryotic expression of the EToV Mpro domain. (Left panel) E. coli M15/pREP4 cells, transformed with pQE-SS-Mpro (lanes 1 and 2) or pQE-SS-Mpro/Gly3304 (lanes 3 and 4), were grown in the presence (+) or absence (–) of 1 mM IPTG for 5 h. Total cell lysates were analyzed in 15% SDS-polyacrylamide gels. Proteins were stained with Coomassie brilliant blue. Positions of the 42-kDa precursor (P42) and the 33-kDa Mpro and 16-kDa internal cleavage products (IC) are indicated. (Right panel) Expression of an EToV Mpro-GST chimera in E. coli. E. coli M15/pREP4 cells, transformed with pQE-SS-Mpro (lanes 1 and 2) or pQE9-SS-Mpro-GST (lanes 3 and 4), were grown in the presence (+) or absence (–) of 1 mM IPTG for 5 h. Total cell lysates were analyzed in 15% SDS-polyacrylamide gels. Proteins were stained with Coomassie brilliant blue. Positions of the 33-kDa Mpro and 16-kDa internal cleavage products are indicated as well as the 26-kDa GST product. wt, wild type.

Although sequence conservation between the putative torovirus M^pro and the M^pros of other nidoviruses is very weak, its sequence could be fitted to existing M^pro alignments (3, 4, 74) in the regions containing the active-site His and Cys/Ser residues. The putative EToV M^pro is predicted to adopt a two-ß-barrel structure with His³³⁰⁴ and Ser³⁴¹⁶ as the main active-site residues and, again, Glu³³⁴⁷ as the most likely candidate for the role of third residue within the catalytic triad (Fig. 1B). From our data, the torovirus M^pro appears to be no more closely related to the coronavirus M^pro than to its roni- and arterivirus homologues. Perhaps most surprising, the torovirus M^pro differs from the M^pros of corona- and roniviruses in that it is not a cysteine proteinase, but rather, like its arterivirus homologue, uses serine as the principal nucleophile.

Proteolytic activity of EToV M^pro. The bioinformatical analyses of the putative EToV M^pro provided a theoretical framework for subsequent experimental studies. The hydrophilic region between HR-1 and -2, which spans the predicted proteinase domain, was expressed in E. coli (Fig. 2). A construct in which the predicted active-site His residue was replaced by Gly was used as a control (Fig. 2B). IPTG-induced expression of these constructs should yield a 42-kDa primary translation product. Indeed, a protein of this size was detected in cells expressing the His-to-Ala mutant. However, in cells expressing the intact proteinase domain, two products with apparent molecular masses of 33 and 16 kDa were found instead. These results suggested that the EToV pp1a region comprising residues 3186 to 3550 indeed contains a functional proteinase domain mediating autocatalytic processing.

The 33- and 16-kDa products were purified from E. coli and N-terminally sequenced by performing 5 or 8 cycles of Edman degradation, respectively. Analysis of the 33-kDa product indicated that cleavage had occurred at the sequence ³²⁴⁶SNFSFQSVFSKAT³²⁵⁸, thus identifying Ser³²⁵² as the N-terminal residue of EToV M^pro (Fig. 3) (Note that, throughout this article, amino acid residues flanking the scissile bond, indicated by , are given from N to C terminus in the single-letter code, where "x" indicates any residue.) The 16-kDa product proved to be a mixture of two protein species. For one of these, the N terminus was identical to that of the 33-kDa product. The other product apparently arose from proteolytic cleavage at an internal sequence, ³³⁹²SEFATQAWQTVN³⁴⁰³(data not shown). Indeed, cleavage of M^pro at this site would cut the proteinase effectively in half, thus giving rise to two equal-size (16.5 kDa) products. These results tentatively identified FxxQ(S, A) as the EToV M^pro substrate consensus sequence (residues are given in parentheses to indicate the variation occurring at a particular position within the cleavage site).

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FIG. 3. Characterization of the N-terminal EToV Mpro autoprocessing site by protein sequencing. The 33-kDa cleavage product, purified from bacterial lysates (Fig. 2B, lane 2), was subjected to Edman degradation. Phenylthiohydantoin (PTH)-amino acids generated during each reaction cycle were detected by their absorbance at 269 nm (expressed as milliabsorption units [mAU]; y axis) and identified by their characteristic retention times (in minutes; x axis) on a reversed-phase high-pressure liquid chromatography support. (A) Chromatogram of PTH-amino acid standards. (B to F) Chromatograms of PTH-amino acids from reaction cycles 1 to 5. Specific peaks are indicated by the single-letter code.

Analysis of the M^pro flanking sequences identified a putative additional cleavage site downstream of the proteinase domain, ³⁵⁴⁰FKKQS³⁵⁴⁴. In the full-length precursor product encoded by plasmid pQE-SS-M^pro, this sequence is located only 5 residues upstream of the C terminus. Hence, cleavage at this site could not be confirmed. As the hydrophobic region HR-2, C-terminally flanking M^pro, might interfere with efficient expression in E. coli, we did not extend the expression product with EToV sequences, but instead designed an M^pro-fusion protein, which contained the predicted cleavage site including the downstream seven residues, linked via a newly introduced proline residue to residues 1 to 226 of GST (Fig. 2A). Expression in E. coli yielded, as anticipated, two major products of 33 kDa and 26 kDa (Fig. 2B), apparently corresponding to mature M^pro and the cleaved-off GST moiety. N-terminal sequence analysis of the 26-kDa product confirmed this notion and indicated that proteolytic cleavage indeed had occurred at the predicted site ³⁵⁴³GlnSer³⁵⁴⁴ (data not shown).

Cleavage at the sites upstream and downstream of the M^pro domain should yield a 33-kDa protein. Accordingly, in lysates from metabolically labeled EToV-infected cells, a product of this size, comigrating exactly with the bacterial cleavage product, was detected by RIPA with M^pro-specific antisera (Fig. 4) (data not shown). The 16-kDa products, however, were not detected in EToV-infected cells.

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FIG. 4. Detection of Mpro in EToV-infected cells. Ederm cells, infected (+) or mock-infected (–) with EToV, were metabolically labeled with [35S]Met plus Cys from 6 to 9 h p.i. Cell lysates were supplemented with SDS to a final concentration of 2% in order to dissociate protein-protein complexes. The lysates were then diluted 10-fold with detergent solution and subjected to RIPA with polyclonal antiserum K274, directed against the C-terminal 17 residues of Mpro (post) or with preserum (pre). Similar results were obtained with polyclonal antisera K158 and K272, directed against a peptide comprising residues 5 through 196 or the N-terminal 17 residues of EToV Mpro, respectively (not shown). The samples were analyzed in 15% SDS-polyacrylamide gels. Molecular size markers are given in kilodaltons. The 33-kDa Mpro species is indicated. High-molecular-mass products—presumably Mpro precursors—are evident at the top of the gel.

Mutagenesis of the predicted EToV M^pro active-site residues. Further analysis of the EToV M^pro was performed by employing the vaccinia virus-based vTF7-3 mammalian expression system (24) (Fig. 5). To this end, residues 10376 to 11472 of the EToV genome were provided with an AUG codon in an optimal context for translation initiation (40) and the resulting ORF was placed under the control of the bacteriophage T7 promoter (Fig. 5A). Expression of this construct predominantly yielded the 33-kDa M^pro species. To assess the importance of the predicted catalytic residues, single-amino-acid substitutions were introduced, and their effects were studied by analyzing the processing activities of the mutant proteinases. Consistent with their proposed catalytic function, replacement of His³³⁰⁴ by either Gly or Arg and of Ser³⁴¹⁶ by Ala completely abolished proteolytic activity. Interestingly, however, an M^pro mutant with a Ser³⁴¹⁶Cys substitution retained partial activity (Fig. 5B).

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FIG. 5. Mutagenesis of predicted active-site residues of EToV Mpro. (A) Mammalian expression constructs for the EToV Mpro domain. The upper panel shows the organization of the C-terminal half of pp1a with hydrophobic regions depicted as gray boxes and the Mpro domain as an oval. The Mpro domain and flanking hydrophilic sequences (represented by a white box) were cloned in pBluescript and placed under the control of the bacteriophage T7 promoter (depicted by the black box and arrow). The relative locations of the predicted active-site His3304 and Ser3416 residues are indicated. White arrowheads indicate Mpro cleavage sites. Also shown schematically are the structure of the P42 precursor and that of the mature 33-kDa Mpro species. (B) vTF7-3 expression of EToV Mpro. OST7-1 cells were infected with recombinant vaccinia virus vTF7-3 and transfected with pBluescript-based expression vectors encoding either the wild-type EToV Mpro (wt) or mutants in which the predicted active-site His3304 and Ser3416 residues had been replaced by Arg or Gly or Cys or Ala, respectively. Mock-transfected cells were taken along as a negative control (m). Cells were metabolically labeled from 5 to 6 h p.i. Cell lysates were subjected to RIPA with a polyclonal antibody directed against Mpro (K158). Precipitates were analyzed in 15% SDS-polyacrylamide gels, and labeled proteins were visualized by fluorography. The positions of the 42-kDa precursor (P42) and of the 33-kDa mature Mpro species are indicated. Molecular masses of marker proteins are given in kilodaltons. (C) Mutagenesis of putative active-site acidic residues. The effect of conservative and nonconservative substitutions of Asp3338, Glu3347, Glu3354, and Asp3358 was assessed in the vTF7-3 system as described above. Amino acid residues are indicated in the single-letter code.

EToV M^pro displays the distinctive traits of a classical serine proteinase, and hence the existence of a third acidic catalytic residue was surmised. On the basis of the alignments (Fig. 1A and B), Glu³³⁴⁷ was considered the most likely candidate to occupy a main chain position equivalent to that of the catalytic Asp residue in chymotrypsin. In addition, Asp³³⁸³, Glu³³⁵⁴, and Asp³³⁵⁸ were selected for mutagenesis. However, the substitution for neither of these residues by Asn or Ala affected proteolytic processing of the 42-kDa M^pro precursor (Fig. 5C). One explanation for this result would be that yet another acidic residue is part of the catalytic triad. Still, the fact that our assay relied on autocatalytic cleavages that may occur in cis posed a caveat. Mutagenesis studies of other serine proteases have shown that the acidic active-site residue is not absolutely required for peptide hydrolysis, although its substitution may cause the enzymatic activity to drop by several orders of magnitude (11, 16, 33, 41, 64, 65). Yet, in an experimental setup in which processing occurs by highly efficient cleavage in cis, even such considerable differences in enzymatic activity may go unnoticed. We therefore designed a more sensitive trans-cleavage assay, outlined in Fig. 6A, which entailed coexpression of enzymatically active M^pro and a substrate protein. Enzyme and substrate were expressed from the same transcript with translation of the latter being driven by the EMCV IRES.

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FIG. 6. Effect of substitutions of possible active-site acidic residues as determined in a trans-cleavage assay. (A) Schematic outline of the trans-cleavage assay. The upper panel shows the structure of the expression constructs with the ORFs encoding the Mpro enzyme and substrate depicted as boxes. The expression of the ORFs was under the control of the T7 promoter (black box and arrow). Translation of the downstream ORF for the substrate was driven by the EMCV IRES (indicated by a black box). For the Mpro enzyme, the relative locations of the active-site His and Ser residues are indicated. Cleavage sites in the Mpro precursor and in the substrate are indicated by white arrowheads. Substrate sequences derived from ORF1a/pp1a and from EToV N are indicated by hatching or dots, respectively. In the substrate, the N-terminal cleavage site was abolished (QSAG) and the enzyme was inactivated by a Ser3416Ala substitution. Shown below are the structures of the various precursor and cleavage products. (B) Mutagenesis of possible active-site acidic residues. The effect of conservative and nonconservative substitutions of Asp3338, Glu3347, Glu3354, and Asp3358 was assessed in the vTF7-3 system essentially as described in Fig. 5. Substitutions are indicated in the single-letter code. Metabolic labeling was from 3.5 to 4.5 h p.i., and RIPA was performed with antisera K270 (-pp1a), K158 (-Mpro), and rabbit anti-EToV N (-EToV N). The positions of the various precursors and mature products are indicated on the right. Molecular masses of marker proteins are given in kilodaltons on the left. Amino acid residues are indicated in the single-letter code. m, mock-transfected negative control; wt, wild type.

The substrate was a 71-kDa chimeric protein consisting of (i) residues 1 to 103 of pp1a/pp1ab, (ii) a EToV M^pro-containing segment consisting of pp1a/pp1ab residues 3187 to 3551, and (iii) residues 2 to 160 of the EToV N protein, as listed from N to C terminus. In this fusion protein, the N-terminal M^pro cleavage site was abolished by a QSAG substitution, while the M^pro was inactivated by changing the active site Ser³⁴¹⁶ to Ala. However, the cleavage site C terminal of M^pro was left intact and hence remained available for proteolytic cleavage in trans. This should give rise to products of 52 kDa (the pp1a-M^pro fusion protein) and of 19 kDa (the cleaved-off N moiety), which are readily distinguishable from the enzymatically active M^pro and its precursors. Processing was monitored by RIPA with antisera against the N terminus of pp1a, M^pro, and the N protein and the effect of substitutions of the selected acidic residues was assessed (Fig. 6B). A construct in which the M^pro enzyme was inactivated by a Ser³⁴¹⁶Ala substitution was taken along as a negative control.

M^pro derivatives, in which Asp³³³⁸, Glu³³⁵⁴, and Asp³³⁵⁸ had been altered, behaved like the wild-type enzyme in the trans-cleavage assay. Substitution of Glu³³⁴⁷, however, reduced proteolytic activity as indicated by accumulation of the 71-kDa noncleaved substrate precursor and of the M^pro precursors of 42 and 34 kDa; the latter protein species apparently represented an intermediate generated by processing of the 42-kDa M^pro precursor at the N-terminal but not at the C-terminal cleavage site (Fig. 6B).

Top Abstract Introduction Materials and Methods Results Discussion References

 
The main proteinases, which mediate most of the processing steps of nidovirus replicase polyproteins, have been studied so far only for corona-, arteri-, and roniviruses. Here, we report the biochemical characterization of the fourth member, the torovirus M^pro. The nidoviral M^pros all belong to a family of viral and cellular proteinases, resembling picornavirus 3C (3C-like proteinases [3CLPs]). Moreover, they are located at cognate positions within the C-terminal half of pp1a, typically flanked by hydrophobic domains at either side (74, 76). Hence, the null hypothesis is that the proteinases of extant nidoviruses have all evolved from a single ancestral proto-nidovirus 3CLP. However, if so, they have diverged to an extreme extent. As noted previously (74, 76), primary sequence diversity of the corona-, roni-, and arterivirus M^pros is so pronounced that even the most sensitive computer-aided methods do not reveal any specific relationship among them that would justify their grouping and separation from other cellular or viral 3CLPs.

Within the order Nidovirales, the toroviruses seem to be most closely related to the coronaviruses (10, 25, 58, 60). We therefore anticipated at the onset of this study that the torovirus M^pro might bridge the large evolutionary gap between the main proteinase of the coronaviruses and those of the other nidoviruses (76). Surprisingly, however, from its primary sequence, the M^pro of EToV Berne seems no more related to the coronaviral proteinase than to those of the arteri- and roniviruses (Fig. 1B). The characteristics of the torovirus M^pro in relation to those of the other nidoviruses are discussed in the paragraphs below.

M^pro-mediated processing and cleavage site specificity. Nidoviral M^pros and related proteinases in other RNA viruses are released from adjoining polyprotein domains by autocatalytic processing (21, 76). Likewise, when pp1a segments, containing the predicted EToV M^pro domain, were heterologously expressed in prokaryotic and in mammalian cells, the proteinase liberated itself by cleaving both at an N-terminal site and at a C-terminal site. This yielded a mature M^pro of 33 kDa, a protein of which size was also detected in EToV-infected cells by RIPA with M^pro-specific antisera. Interestingly, in EToV-infected cells, autocatalytic release of M^pro might be inefficient as during a 3-h continuous metabolic labeling period a considerable proportion of the proteinase seemed to remain part of a large precursor (Fig. 4). Similar observations were reported for the arteri- and coronavirus M^pros (32, 54, 63, 71). It has been suggested, that the long-lived M^pro intermediates are membrane associated via the flanking hydrophobic domains. Anchoring of proteinase precursors to intracellular membranes might well be a central phenomenon in nidovirus polyprotein processing and/or replication (39, 54, 71).

N-terminal sequence analysis of mature EToV M^pro showed that autocatalytic cleavage occurred at the location ³²⁴⁶SNFSFQSVFS³²⁵⁵. The sequence ³⁵³⁸QPFKKQSVSN³⁵⁴⁷was identified as the C-terminal cleavage site. Unexpectedly, in prokaryotic cells, processing occurred also at a site internal to M^pro, ³³⁹²SEFATQAWQT³⁴⁰¹, effectively cleaving the proteinase in half. It is tempting to speculate that, during EToV infection, M^pro might inactivate itself as part of a feedback autoregulatory mechanism or, otherwise, that processing at the internal site gives rise to an alternative cleavage pathway (71). However, we have no evidence that internal processing actually occurs in mammalian cells. The 16-kDa cleavage products were detected neither in the vTF7-3 expression system nor in EToV-infected cells. Hence, it cannot be excluded that internal cleavage, as observed in E. coli, is an artifact resulting from overexpression and possibly aided by protein misfolding, which might have exposed cleavage sites that are normally inaccessible. Intriguingly, however, the internal cleavage site is also conserved in BToV M^pro (22).

Catalytic center and substrate specificity. Although sequence identity between EToV M^pro and its nidovirus homologues or other viral and cellular chymotrypsin-like enzymes is limited, sequence alignments clearly implicated Ser³⁴¹⁶ and His³³⁰⁴ as the main catalytic residues. Consistent with this notion, their replacement by Ala and by Gly or Arg, respectively, abrogated enzymatic activity. The M^pros of corona- and roniviruses (2, 73, 74), like the hepatitis A virus 3C proteinase (1, 7), employ a catalytic Cys-His dyad within the context of the chymotrypsin-fold. Under the assumption that the EToV M^pro is a classical serine proteinase, a third acidic catalytic residue was expected (20). Although sequence alignments of EToV M^pro with other proteinases were far from robust, particularly in the region that should contain this third residue, our analyses suggested Glu³³⁴⁷ as the most likely candidate. However, neither substitution mutagenesis of Glu³³⁴⁷ nor that of the proximal Asp³³³⁸, Glu³³⁵⁴, and Asp³³⁵⁸ noticeably affected autocatalytic release of M^pro in heterologous expression studies. Yet, in an assay that tested for processing in trans, the efficacy of M^pro cleavage of an artificial substrate was clearly reduced by substitution of Glu³³⁴⁷, but not by that of the other acidic residues. Although our findings do not prove that Glu³³⁴⁷ is included in a catalytic triad with Ser³⁴¹⁶ and His³³⁰⁴, they would at least be consistent with this notion. This view might seem at odds with observations made for various other viral and cellular chymotrypsin-like proteinases, where site-directed mutagenesis of the third residue resulted in a far more dramatic loss of proteolytic activity (11, 16, 33, 41, 64, 65). Still, in the case of severe acute respiratory syndrome (SARS) coronavirus M^pro, replacement of the active-site Cys by Ser yields a functional enzyme. Although this mutant proteinase relies exclusively on a Ser-His catalytic dyad, its activity is merely 40-fold reduced as compared to that of wild-type SARS coronavirus M^pro (36). A reduction in activity of this magnitude might have only a modest effect on processing even in our trans-cleavage assay under conditions of vTF7-3-driven EToV M^pro overexpression. As the mapping of active-site residues by the combination of comparative sequence analysis and site-directed mutagenesis is inherently fraught with a measure of uncertainty, definitive answers with respect to catalytic center composition and the presence/identity of a third catalytic residue will require the elucidation of the torovirus M^pro crystal structure.

Comparison of the sequences flanking the scissile bonds of the internal and the N- and C-terminal cleavage sites tentatively identifies FxxQ(S, A) as the substrate consensus sequence of EToV M^pro. Its cleavage site specificity thus resembles that of other nidoviral M^pros, which, as is typical for 3CLPs, all require Gln or Glu at the P1 position (74, 76). The specificity for P1-(Gln, Glu) of the picorna-, arteri-, and coronavirus enzymes is determined by a strictly conserved His, which via its imidazole side chain hydrogen bonds to the carbonyl/carboxylate oxygens of the P1 side chain (1, 2, 4, 7, 44, 45, 47, 73, 74, 76). A corresponding His residue is also present in the torovirus M^pro (EToV His³⁴³⁰) as part of a Gly-X-His sequence (Fig. 1B), a motif well conserved in most 3CLPs (including arteri- and ronivirus M^pro), but saliently absent in the M^pros of coronaviruses; the latter have a Tyr-Met-His motif instead (2, 4, 34, 64, 74, 75). In many 3CLPs, conserved Ser/Thr residues, located five residues upstream of the catalytic Ser/Cys, are also part of the substrate-binding subsite S1 and assist in binding by forming additional hydrogen bonds with the carbonyl/carboxylate oxygen atoms of the P1 side chain (4, 44, 47, 48, 74). We propose that, in the torovirus M^pro, Thr³⁴¹¹ plays a similar role. This would again be a difference from the coronavirus M^pro, which lacks a corresponding Ser/Thr residue (2, 74).

The arteri- and ronivirus M^pros prefer glutamic acid at the P1 position of their substrates, whereas coronavirus M^pro requires glutamine (64, 74, 76). In arterivirus M^pros, this substrate preference is presumably conferred by a Ser residue (located three residues downstream of the S1 subsite His; S¹³⁷ in EAV M^pro; see Fig. 1B), which would hydrogen bond with the carboxylate oxygen atom (that is, the one not interacting with the subsite S1 His/Thr pair) of the P1-Glu side chain (4). This Ser is not conserved in the corona- and torovirus M^pros; instead, at the corresponding positions, Glu and Leu residues, respectively, are found (Fig. 1b). The S1 specificity site of coronavirus M^pro consists of the main chain atoms of Met¹⁶⁵, Glu¹⁶⁶, and His¹⁷² and the side chains of Phe¹⁴⁰ and His¹⁶³, with the imidazole of the latter residue interacting with the P1-Gln side chain (2, 3, 73) (residue numbering according to SARS-CoV M^pro). Also with respect to S1 subsite composition, the torovirus main proteinase differs from that of coronaviruses. Although EToV M^pro, like its coronavirus homologues, apparently prefers P1-Gln, none of the coronavirus S1 subsite residues are conserved, except for His¹⁶³. As yet, it is not clear from the EToV M^pro sequence how the P1-Gln is accommodated.

Tentative M^pro processing scheme of torovirus pp1a/pp1ab. Although each of the three established EToV M^pro cleavage sites conforms to the consensus FxxQ(S, A), we believe, on the basis of alignments of pp1a/pp1ab of coronaviruses and the toroviruses EToV and BToV, that Tyr/Met/Leu and Gly/Lys may also be tolerated at the P4 and P1' positions, respectively. Although the picture is still incomplete, the substrate specificity of the torovirus M^pro is reminiscent of and yet distinct from those of the corona-, arteri-, and roniviruses, which mainly conform to LQ(S, A), E (G, S, A), and VxHE(L, V), respectively (74, 76). In particular, a preference for a bulky hydrophobic residue at P4 and no apparent predilection for certain residues at P2 would give the EToV M^pro a unique cleavage site formula. A tentative M^pro processing scheme of EToV pp1a/1b is presented in Fig. 7, with the sequences and locations of potential cleavage sites listed in Table 2. Several points are of note. (i) All cleavage sites predicted for EToV are conserved in BToV (22). (ii) A putative cleavage site, ²⁸⁷⁰FKKQSV²⁸⁷⁵ (Table 2, site 1), identical in sequence to the one C terminal of the M^pro domain (Table 2, site 4), is found halfway in EToV pp1a at a position topologically similar to that of an accessory papain-like proteinase 2 site within coronavirus pp1a. (iii) Of the predicted sites in the ORF1b-encoded part of the replicase (Table 2, sites 10 to 14), only one, located between the RdRp and zinc finger/helicase domains, conforms to the proposed consensus FxxQ (S, A) sequence (site 10; Table 2). Future studies should determine whether the predicted sites within pp1a/pp1ab are actually cleaved by M^pro. (iv) At the very C terminus of torovirus pp1a, there is a domain that is absent from all other nidovirus pp1a proteins and that shares identity with a predicted cyclic phosphodiesterase (CPD) motif in the ns2A protein of group 2 coronaviruses and in the rotavirus VP3 guanylyl transferase (Fig. 7) (57, 60). Puzzlingly, a cleavage site C terminal of this domain is not immediately apparent, raising the question whether M^pro utilizes a noncanonical site, whether another viral or host proteinase is involved, or whether processing of pp1ab yields an RdRp with the CPD homologue attached; note that in the latter case, processing of pp1a would still produce an additional, "free" CPD.

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FIG. 7. Comparisonof the pp1a/pp1ab domain organization in different nidoviruses and a tentative Mpro processing scheme of the torovirus replicase polyproteins. The C-terminal half of pp1a (dark gray) and the ORF1b-encoded part of pp1ab (light gray) are shown schematically, to scale, for corona-, toro-, arteri-, and roniviruses. The border between amino acids encoded in ORF1a and ORF1b is indicated as RFS (ribosomal frameshift). The locations of domains that have been identified as structurally or functionally related are highlighted and indicated as follows: TM, putative transmembrane domains; Mpro, main proteinase; RdRp, RNA-dependent RNA polymerase motif; Z, zinc finger motif; Hel, helicase; Exo, (putative) 3'-to-5' exonuclease (ExoN); N, uridylate-specific endoribonuclease (NendoU); MT, (putative) 2'-O-methyl transferase (26, 30; see also reference 57 and references therein). Also indicated is the (predicted) cyclic phosphodiesterase domain (CPD) that resides near the C terminus of the torovirus pp1a. Arrowheads represent known cleavage sites for accessory papain-like proteinase (cyan) or Mpro (red), as established for corona-, arteri-, and roniviruses and as established casu quo predicted here for toroviruses (see also Table 2). The figure was adapted from reference 56.

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TABLE 2. Tentative cleavage sites in pp1a/pp1ab for the torovirus main proteinase

Evolutionary implications. EToV M^pro combines several traits of its closest relatives. (i) As is typical for nidovirus M^pros, the EToV proteinase has a predicted three-domain structure, with two catalytic ß-barrel domains and an additional C-terminal domain of unknown function. (ii) With respect to substrate specificity, the EToV M^pro resembles its coronavirus homologue in its preference for P1-Gln. (iii) Then again, it has what appears to be a canonical substrate-binding subsite, S1, resembling that of arteri- and ronivirus M^pros, but clearly distinct from that of coronavirus M^pro. (iv) Finally, in contrast to the M^pros of corona- and roniviruses, but like that of arterivirus, the torovirus M^pro uses serine instead of cysteine as its principal nucleophile. Rather than clarifying the evolutionary history of the nidoviral M^pros, the analysis of a torovirus M^pro seems to make the picture even more complex. If anything, our findings further emphasize the unique properties of the coronavirus M^pro, which on the basis of its catalytic system and substrate-binding pocket, was already considered an outlier among viral and cellular chymotrypsin-like homologues (2, 74). It is still quite possible, however, that striking similarities between corona- and toroviral M^pros will become overt once the crystal structure of toroviral M^pro has been solved.

Corona- and toroviruses share many traits (e.g., with regard to virion composition, genome organization, and the extent of colinearity in the ORF1b-encoded region of pp1ab), which would justify their grouping together, separate from the arteri- and roniviruses (15, 19, 25, 26). However, in a recent study of Gonzalez et al. (25), entailing a systematic quantitative analysis of sequence conservation among nidoviral proteins, the expected sequence affinity between corona- and toroviruses was not evident. Thus, with the topology of the nidovirus tree undecided, it was suggested that "the nidovirus phylogeny must be verified later when the number and diversity of torovirus and ronivirus sequences will match those of arteriviruses and coronaviruses" (25). If it were to be firmly established that of the nidoviruses, corona- and toroviruses are, after all, the most closely related, and if this evolutionary relationship also holds for the M^pro (i.e., if no RNA recombination-based exchange of proteinase domains—or parts thereof—has occurred during nidoviral divergence), our observations would have one more major implication: namely that the transition from serine- to cysteine-based proteolytic catalysis (or vice versa) has happened more than once in the course of nidovirus evolution. In this respect, it is of interest that a mutant EToV M^pro with a Ser³⁴¹⁶Cys substitution retained enzymatic activity and that, conversely, the catalytic site CysSer substitution in SARS-CoV M^pro also yields an active enzyme (36).

 
We acknowledge the contribution of Alexander E. Gorbalenya to the bioinformatical analysis of EToV ORF1a-derived cDNA clones 133 and 135 and EToV pp1a, as well as to the design and analysis of some of the experiments. We are grateful to Peter J. M. Rottier and Jolanda D. F. de Groot-Mijnes for critical reading of the manuscript.

 
* Corresponding author. Mailing address: Virology Division, Department of Infectious Diseases and Immunology, Faculty of Veterinary Medicine, Utrecht University, 3584 CL Utrecht, The Netherlands. Phone: 31 30 2531463/2485. Fax: 31 30 2536723. E-mail: R.Groot{at}vet.uu.nl.

Top Abstract Introduction Materials and Methods Results Discussion References

 

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Journal of Virology, April 2006, p. 4157-4167, Vol. 80, No. 8
0022-538X/06/$08.00+0     doi:10.1128/JVI.80.8.4157-4167.2006
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