| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
|
|
|
|||||||
|
|||||||||
1 Unité des Virus Emergents EA3292, EFS Alpes-Méditerranée and Faculté de Médecine de Marseille, 27 Boulevard Jean Moulin, 13005 Marseille cedex 5, France
2 Department of Biological Oceanography, Royal Netherlands Institute for Sea Research, NL-1790 AB Den Burg, The Netherlands
Correspondence
Houssam Attoui
h-attoui-ets-ap{at}gulliver.fr or
houssam.attoui{at}medecine.univ-mrs.fr
 |
ABSTRACT |
|---|
 TOP ABSTRACT INTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
The GenBank/EMBL/DDBJ accession numbers for the sequences described in this paper are DQ126101 [GenBank] –DQ126111 [GenBank] .
A supplementary table showing sequences of RdRp used in phylogenetic analysis of Micromonas pusilla reovirus is available in JGV Online.
|
INTRODUCTION |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
30 tentative species reported to date (Mertens et al., 2005
). The family currently includes 12 distinct genera, which are Orthoreovirus, Orbivirus, Rotavirus, Coltivirus, Aquareovirus, Cypovirus, Fijivirus, Mycoreovirus, Phytoreovirus, Oryzavirus, Seadornavirus and Idnoreovirus (Mertens & Diprose, 2004; Mertens et al., 2005). Recently, three new genera were proposed to the International Committee on Taxonomy of Viruses (ICTV) for classification of a nine-segmented insect virus, 12-segmented crustacean viruses and an 11-segmented protist virus (described in this paper). These proposals received preliminary support from ICTV.
The morphology of some members of the family Reoviridae has been studied intensively (Prasad et al., 1988; Yeager et al., 1990, 1994; Grimes et al., 1998; Gouet et al., 1999; Hill et al., 1999; Reinisch et al., 2000; Diprose et al., 2001; Nason et al., 2004). The virus particles have icosahedral symmetry with a diameter of approximately 60–85 nm. They are usually regarded as non-enveloped, although some can acquire a transient membrane envelope during morphogenesis or cell exit (Murphy et al., 1968; Estes & Cohen, 1989; Martin et al., 1998; Mertens et al., 2000; Owens et al., 2004). Reoviruses can contain one, two or three concentric protein layers, identified here as ‘subcore’, ‘core’ and ‘outer capsid’, respectively. The inner-capsid layers and proteins are primarily involved in virus assembly and replication and show a remarkable degree of structural conservation between different genera, exemplified by the subcore shell, constructed from 120 molecules of a single protein (Grimes et al., 1998; Reinisch et al., 2000; Mertens, 2004). In contrast, the outer-capsid proteins, which are involved in virus transmission, cell attachment and penetration, show greater variation, reflecting differences in the targeted host species, as well as responses to immune selective pressure by ‘neutralization’ antibodies.
Members of the family Reoviridae can be subdivided into two groups. The ‘turreted’ viruses have 12 icosahedrally arranged projections (called turrets) situated on the surface of the icosahedral core particle, one at each of the fivefold axes (e.g. orthoreoviruses or cypoviruses) (Baker et al., 1999; Hill et al., 1999). The cores of the ‘non-turreted’ viruses have a ‘protein-bilayer’ structure, with a smooth or bristly surface appearance (e.g. rotaviruses or orbiviruses; Grimes et al., 1998; Baker et al., 1999; Mertens et al., 2000, 2005).
An 11-segmented dsRNA virus has been isolated from the marine protist Micromonas pusilla (Brussaard et al., 2004) and the isolate was originally designated Micromonas pusilla RNA virus (MpRNAV). This virus was renamed and is now recognized as Micromonas pusilla reovirus (MpRV). Although 11-segmented dsRNA viruses infecting aquatic animals are known (belonging to the genus Aquareovirus), the isolation of a dsRNA virus from M. pusilla constitutes the first case of isolation of a reovirus from a protist. The polysegmented dsRNA genome of MpRV identified it as a member of the family Reoviridae (Brussaard et al., 2004). Among various algal species, including different strains of M. pusilla, this virus was found to replicate only in strain LAC38 of M. pusilla. We report here a molecular study of MpRV. Sequence and phylogenetic analyses show clearly that MpRV does not belong to any of the genera identified to date.
|
METHODS |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
; Cottrell & Suttle, 1991) at 15 °C under white light as described previously (Brussaard et al., 2004). Algal suspension (20 l; 2x107 cells ml–1) was infected with MpRV and incubated at 15 °C until complete lysis occurred after 1 week.
Viruses were concentrated by ultrafiltration on Vivaflow 200 (molecular weight cut-off, 30 kDa; Vivascience), after which Tween 80 was added to a final concentration of 0·007 %. The viruses were subsequently partially purified by removing cell debris from fresh lysate using low-speed centrifugation at 7000 g for 30 min at 4 °C. The supernatant was decanted and viral particles were concentrated by ultracentrifugation at 100 000 g for 2 h at 8 °C using an SW28 rotor. The viral pellets were resuspended in 150 µl SM buffer [0·1 M NaCl, 8 mM MgSO4, 50 mM Tris/HCl (pH 7·5), 0·005 % (w/v) glycerol; Wommack et al., 1999] and stored at 4 °C until use.
Virus purification and electron microscopy.
MpRV particles were purified by layering the suspension onto a preformed linear Percoll (Amersham Biosciences) gradient in a dilution buffer [150 mM NaCl, 250 mM sucrose, 1 mM MgCl2, 4 mM CaCl2, 10 mM Tris/HCl (pH 8·0)] followed by centrifugation at 110 000 g (45 min, 10 °C). The virus band was recovered and processed as described previously (Mohd Jaafar et al., 2005). These particles were subsequently purified on a discontinuous caesium chloride gradient (40/55 %) as described by Burroughs et al. (1994), at 10 °C for 2 h at 210 000 g.
Cores of MpRV were prepared by treating 100 µl Percoll-purified virus with 100 µl CaCl2 (3 M; final concentration, 1·5 M) (Estes & Cohen, 1989) for 30 min at 37 °C. The cores were then purified on the 40/55 % discontinuous caesium chloride gradient as described above. MpRV core particles were recovered at the interface, diluted with an equal volume of 100 mM Tris/HCl (pH 8·0) and processed for electron microscopy.
The virus was adsorbed onto Formvar/carbon-coated grids, stained with 2 % potassium phosphotungstate for 30 s and dried prior to being examined by electron microscopy using a Philips Morgagni 268 transmission electron microscope.
Isolation and purification of the genomic dsRNA for cloning.
Virus dsRNA was extracted from the suspended viral concentrate by using a commercially available guanidinium isothiocyanate-based procedure (RNA NOW reagent; Biogentex). Briefly, samples (150 µl) were dissolved in 1 ml reagent by vigorous mixing. Chloroform (200 µl) was added and the mixture was shaken for 1 min and kept for 10 min on ice, followed by centrifugation at 12 000 g for 10 min at 4 °C. The supernatant was recovered, mixed with 900 µl 100 % 2-propanol and incubated overnight at –20 °C. The RNA was pelleted by centrifugation at 18 000 g for 10 min at 4 °C, washed with 75 % ethanol, dried and dissolved in 50 µl water. The dsRNA was further purified by precipitating high-molecular-mass single-stranded RNAs in 2 M LiCl, as described elsewhere (Attoui et al., 2000a).
Cloning of the dsRNA segments.
The genome segments of MpRV were copied into cDNA, cloned and sequenced according to the single-primer amplification technique described previously (Attoui et al., 2000a, b). Briefly, the viral dsRNA was separated on 1 % agarose gel and purified by using an RNaid kit (Bio 101). A previously described 3'-amino-blocked oligodeoxyribonucleotide (Attoui et al., 2000a, b) was ligated to both of the 3' ends of the purified dsRNA segments by using T4 RNA ligase, followed by reverse transcription and PCR amplification using a complementary primer. PCR amplicons were analysed by agarose-gel electrophoresis, ligated into the pGEM-T cloning vector (Promega) and transfected into competent XL-Blue Escherichia coli. Insert sequences were determined by using M13 universal primers, a D-rhodamine DNA sequencing kit and an ABI Prism 377 sequence analyser (Perkin Elmer).
Assays of virus replication in insect-, mammalian- and fish-cell lines.
The virus was inoculated into the fish-cell line FHM (fathead minnow), which was grown in Leibovitz's L-15 medium at 28 °C. The inoculated FHM cells were incubated at either 20 °C (a temperature which is closer to the growth temperature of MpRV in M. pusilla) or 28 °C.
Other cell lines tested included mosquito-cell lines and mammalian-cell lines. The mosquito-cell lines C6/36 and AA23 (both from Aedes albopictus), A20 (Ades aegypti), AE (Aedes aegypti) and A w-albus (Aedes w-albus) were all grown in Leibovitz's L-15 medium at 28 °C. The inoculated cells were incubated at either 20 or 28 °C. The mammalian-cell lines L-929 (mouse fibroblast), BHK-21 (hamster kidney), BGM (monkey kidney), HEp-2 (human adenocarcinoma) and MRC5 (human embryo lung) were all grown at 37 °C in Eagle's minimal essential medium supplemented with 5 % fetal bovine serum. The inoculated cells were incubated at either 37 or 32 °C (a lower temperature, as MpRV grows at low temperature in M. pusilla).
For the purpose of adsorbing the virus to the cells, 100 µl MpRV concentrate was added to the cell monolayers in a 25 cm2 flask and incubated at 28 °C (mosquito or fish cells) or at 37 °C (mammalian cells) for 1 h. The cell were washed twice with PBS and the culture medium was added. At day 5 post-infection (p.i.), the cells were scraped and half of the scraped-cell suspension was pelleted. The supernatant was discarded and the RNA was extracted by using RNA NOW (Biogentex). An aliquot of the remaining scraped-cell suspension was used to infect fresh cells in a second passage. Two more passages were subsequently performed.
The extracted RNA was processed for agarose-gel electrophoresis and RT-PCR, using specific MpRV primers as described below.
RT-PCR of the RNA extract from the cell lines.
The RNA was copied into cDNA by using random hexanucleotide primers as described previously (Attoui et al., 1998). Briefly, the RNA was denatured in 15 % DMSO by heating at 99 °C for 1 min and incubated immediately on ice. Reverse transcription was performed by using Superscript III reverse transcriptase (Invitrogen) at 42 °C. The resulting cDNA was PCR-amplified using first-round primers MpRVSeg2s1 (forward, positions 2259–2284: 5'-CACGCGCACGCAACGTTCTTATAGAC-3') and MpRVSeg2r1 (reverse, positions 2758–2733: 5'-CGTACACTGATCTAATGCGTAACATG-3') to produce an amplicon of 500 bp, and second-round primers MpRVSeg2s2 (forward, positions 2337–2362: 5'-AGCTGGATTCTCATGGTCAATAGCGG-3') and MpRVSeg2r2 (reverse, positions 2636–2611: 5'-CAGCGTCTGTAGCAATAACCTCGCGC-3') to produce an amplicon of 300 bp.
Sequence analysis and phylogenetic comparisons.
Analysis of the MpRV sequence was performed by comparing each segment sequence with a database constructed with all available sequences from the family Reoviridae, using the local BLAST program implemented in the DNATools package (version 5.2.018; Rasmussen, 1995).
The predicted sequences of the proteins encoded by the 11 segments were also analysed by using the NCBI's online BLAST program (http://www.ncbi.nlm.nih.gov/blast/).
For phylogenetic analysis, the putative RNA-dependent RNA polymerase (RdRp) sequence of MpRV was compared with the amino acid sequences of putative RdRps of representative strains of viruses representing the 12 genera of the family Reoviridae. GenBank accession numbers are provided in Supplementary Table S1 (available in JGV Online). Sequence alignments were performed by using the CLUSTAL W (version 1.84) software program (Thompson et al., 1994). Phylogenetic analyses were carried out with the software program MEGA3 (Kumar et al., 2004) using the Poisson-correction or the gamma-distribution algorithms and the neighbour-joining method for tree building.
|
RESULTS |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
15 nm thick) surrounding a more compact internal structure (75 nm).
The particles that were purified on CsCl have a mean diameter of 75 nm (Brussaard et al., 2004), which suggests that these particles had lost the outermost thin layer of protein. However, this size is similar to that described for whole particles of other viruses of the family Reoviridae.
Particles that had been treated with CaCl2 and purified on a Percoll gradient had a diameter of 50 nm, showing that they had lost outer capsid proteins. They also had a smooth outline (Fig. 1), similar to that observed for the subcores (the pseudo-T=2, also known as modified T=1, layer) of rotaviruses, orbiviruses and seadornaviruses (Mertens et al., 2005; Mohd Jaafar et al., 2005), which are non-turreted viruses.
|
) were all cloned, sequenced and deposited in GenBank under accession numbers listed in Table 1. The lengths of the segments and their corresponding encoded proteins are shown in Table 1. Analysis of the 5' and 3' non-coding regions (NCRs) showed that all of the segments share five conserved nucleotides at their 5' ends and six conserved nucleotides at their 3' ends (5'-GAAGA----AAAGUC-3'; Table 1). Moreover, the first and last 2 nt of all of the segments are inverted complements.
|
|
).
The usual size of segment 1 (Seg-1) for viruses of the family Reoviridae is approximately 4000 bp. The Colorado tick fever virus (CTFV) genome has previously been reported to have the largest Seg-1 of all sequenced reoviruses (4350 bp; Attoui et al., 2005). The Seg-1 of MpRV determined in this study was found to be 5792 bp long, which is unusually longer than any Seg-1 in other members of the family Reoviridae. Sequence analysis of MpRV Seg-1 showed that it contains a single open reading frame (ORF) encoding the VP1 protein, which is 1897 aa long.
The BLAST search showed that vp1 exhibited significant homology (as indicated by the e values of the BLAST program) to viral, bacterial and yeast haemagglutinins. This analysis showed that aa 88–321 exhibited 24 % identity with the minor capsid protein sigma-1 of orthoreoviruses (a haemagglutinin responsible for cell attachment; GenBank accession number AAA47276 [GenBank] ).
It is noteworthy that VP1 was found to be related to various haemagglutinins, such as those of the bacterial pathogens Burkholderia spp. (amino acid identity, 20 %; similarity, 40 %; E value, 4x10–6) and Staphylococcus spp. (amino acid identity, 19 %; similarity, 38 %; E value, 3x10–4) and the yeasts Candida albicans (identity, 20 %; similarity, 39 %; E value, 3x10–4) and Saccharomyces cerevisiae (identity, 20 %; similarity, 37 %; E value, 7x10–6). VP1 also matched the envelope proteins of viruses such as those of equine herpesvirus gp2 (identity, 20 %; similarity, 32 %) or that of Acholeplasma bacteriophage (identity, 26 %; similarity, 46 %).
It is interesting to note that VP1 has a high serine and threonine content (
11 % of each), compared with 1–7·5 % for other amino acids. This is characteristic of glycoproteins and, in particular, for mucin and mucin-like proteins (Byrd & Bresalier, 2004) and cell-wall adhesins. Such serine- and threonine-rich proteins are usually heavily O-glycosylated. In summary, VP1 might form an extra coat at the outermost surface.
Amino acid sequence repeats were identified within VP1. Interestingly, each repeat was found to align best with a protein sequence immediately N-terminal to it in VP1. The repeated sequences were not identical to the matching sequences. This is evocative of what has been described as sequence duplication in viral genes, followed by distinct evolution of the parental and the daughter repeated sequences (Gibbs & Keese, 1995). Examples of such repeats are shown in Fig. 3.
|
The VP3 (Seg-3) of MpRV might represent the pseudo-T=2 (also known as modified T=1) layer of the virus, i.e the subcore layer. It was found to partially match (aa 229–311; identity, 26 %) the P3(T2) of Rice dwarf virus (genus Phytoreovirus) and the lambda-1 (T=2 protein) of Mammalian orthoreovirus MRV3 (aa 50–145; identity, 20 %). Interestingly, lambda-1 of MRV3 possesses NTPase and helicase activities (Mertens et al., 2005).
The VP5 of MpRV was found to partially match (aa 214–318; identity, 21 %) the outer-capsid spike protein VP4 of Rotavirus A. It also showed 24 % identity to the killer toxin protein (GenBank accession no. S51548) of yeast M28 dsRNA virus (an unclassified virus). Segment 5 shows an ORF spanning nt 44–2005. This ORF is interrupted by an in-frame TGA stop codon at position 1571–1573. A similar situation has been described in segment 9 of CTFV (genus Coltivirus), in which a read-through has been identified. The occurrence of a read-through in segment 5 of MpRV remains to be identified experimentally by cloning segment 5 in a eukaryotic expression vector under the control of a strong promoter and identification of possible long and short forms of the proteins, as has been realized for CTFV segment 9 (Mohd Jaafar et al., 2004).
The VP7 of MpRV was found to partially match (aa 130–209; identity, 32 %) the non-structural protein NS1 of Cypovirus 1, whereas the VP8 of MPRV partially matched (aa 42–66; identity, 28 %) the NSP2 of human Rotavirus A (NSP2 has a dsRNA helix-destabilization activity, binds RNA and is an NTPase).
The VP9 was found to partially match (aa 269–338; identity, 28 %) the segment 7-encoded protein of Nilaparvata luguens reovirus (a fijivirus), which is a core protein and possesses a nucleotide-binding activity (Mertens et al., 2005).
The proteins VP4, VP6, VP10, VP11 and VP12 did not show any significant match with reovirus proteins.
To summarize, based on sequence comparisons with genomes of members of the family Reoviridae, putative functions deduced from the best-fit analyses were attributed to the various MpRV proteins and the information is presented in Table 2.
|
30 % in the polymerase sequence is suitable to distinguish between genera of the family Reoviridae (Attoui et al., 2002a). However, there are two exceptions to this rule. The first is the rotavirus B polymerase, which is only 22 % identical to other rotaviruses. However, the inclusion of Rotavirus B within the genus Rotavirus together with Rotavirus A and Rotavirus C does not rely primarily on genetic distances between the polymerases of these viruses. It was based on the morphological resemblance between these viruses and the type of disease that they cause. The second exception is the aquareoviruses and orthoreoviruses, which are 42 % identical (Attoui et al., 2002a). This significantly high amino acid identity is evidence of a common ancestry. However, the distinct hosts and the different econiches of these viruses justify their classification within two distinct genera.
The results of the polymerase sequence analysis of MpRV are illustrated by a radial neighbour-joining tree (Fig. 4). MpRV does not cluster with any of the known, characterized members of the family Reoviridae. It clustered with neither aquareoviruses (11-segmented), which are turreted viruses, nor with rotaviruses (11-segmented), which are non-turreted. Rather, MpRV stands as a representative of a separate phylogenetic group. This is confirmed by the low amino acid identity values (5–21 %) between MpRV polymerase and those of member viruses of other genera of the family Reoviridae.
|
|
DISCUSSION |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
), the identification of the 11-segmented dsRNA profile of its genome, the morphological characteristics of the virions and its physicochemical properties led to the classification of MpRV as a tentative member of the family Reoviridae. The present study provides several additional arguments for the classification of MpRV as a full member of the family Reoviridae. Full characterization of the dsRNA genome by cloning and sequencing revealed that it has a total length of 25 563 bp. This is similar to the genome length of other viruses of the family Reoviridae, which range between 18 500 and 29 210 bp (Attoui et al., 2002b; Mertens et al., 2005). However, segment 1 of MpRV is significantly longer than segments 1 of other sequenced members of the family Reoviridae. In addition, the putative polymerase of MpRV partially matches rotavirus polymerase and contains the signature motifs of putative RdRps of viruses belonging to the family Reoviridae. In compliance with the criteria defining the family Reoviridae, analysis of the terminal sequences revealed that all 11 segments of MpRV have conserved termini within the 5' and 3' NCRs. Such terminal sequences are recognized as one of the defining species parameters within the family Reoviridae. These conserved termini in the MpRV genome are different from any of those described previously within the family Reoviridae, showing that MpRV does not belong to any previously described species within this family.
The 11-segmented genome is a characteristic of rotaviruses and aquareoviruses within the family Reoviridae. Being isolated from an aquatic organism, it would be reasonable to suppose that MpRV is a tentative member of the genus Aquareovirus (infecting fishes, crustaceans and molluscs). As an aquatic reovirus, it would be interesting to know whether this virus can infect other aquatic species and whether it has only one host, or whether M. pusilla might represent a vector that transmits the virus among other aquatic species. Our results indicated that MpRV does not replicate in fish-, insect- or mammalian-cell lines that were tested and that it is a member of neither the genus Aquareovirus nor the genus Rotavirus, as MpRV has features unique among the family Reoviridae.
Phylogenetic analysis based on the polymerase amino acid sequence, for example, demonstrated clearly that MpRV is not a member of the genera Rotavirus or Aquareovirus, despite its genome being made of 11 dsRNA segments. Amino acid identity of the polymerase of MpRV is 8–10 % with aquareovirus polymerase and 19–21 % with rotavirus polymerase. These are values comparable to those found between viruses belonging to distinct genera of the family Reoviridae. The morphology of the particles is also not identical to that of other members of the family Reoviridae. The diameter of whole particles purified under conditions not affecting the integrity of the outer coat is significantly larger (90–95 nm) than the diameters usually observed in viruses of the family Reoviridae. In a previous study, when MpRV was purified on a CsCl density gradient, two virus bands were visible (Brussaard et al., 2004). The less-dense virus band was found to contain eight structural proteins, including traces of a protein at approximately 200 kDa that was absent from the denser virus band, suggesting that this protein is removed at high ionic strength. This size is compatible with the deduced size of VP1 of MpRV. This protein is likely to be responsible for the unusually large size of the whole virus particles. VP1 showed similarities within its amino-terminal sequence to Sigma-1 (a haemagglutinin and cell-attachment protein) of MRV (genus Orthoreovirus). This suggested that VP1 might represent the virus attachment protein to the cell wall of M. pusilla. VP1 was also found to exhibit similarities to glycoproteins of viral and non-viral agents. The high serine and threonine content of VP1 suggests that it might be O-glycosylated, as is the case of mucin and mucin-like proteins.
Transient envelope structures have been described for orbiviruses (Martin et al., 1998; Owens et al., 2004), coltiviruses (Murphy et al., 1968; Attoui et al., 2002b), rotaviruses (Estes & Cohen, 1989) and seadornaviruses (Mohd Jaafar et al., 2005) as a consequence of budding of virus particles from the cell membrane or budding into the endoplasmic reticulum during morphogenesis. If MpRV VP1 forms such a structure, MpRV would be the first member of the family Reoviridae to possess a constitutive additional outer coat. This requires further investigation by techniques such as cryoelectron microscopy.
The length of the VP1 of MpRV is unusual among sequenced members of the family Reoviridae. The presence of many repeats within this sequence evokes the possibility that VP1 could have arisen from amino acid fragment duplication, which diverged afterwards. The precise mechanism and the constraints that have driven such an evolution are unknown.
The existence of the remaining seven structural proteins in the purified MpRV particles (Brussaard et al., 2004) is compatible with that described for non-turreted reoviruses, where particles are composed of seven structural proteins, such as in seadornaviruses and orbiviruses (Mertens et al., 2005; Mohd Jaafar et al., 2005). The MpRV particles that were treated with CaCl2 generated structures that could be compared with the smooth, non-turreted subcore layer of orbiviruses, indicating that MpRV belongs to the non-turreted group within the family Reoviridae. This is further evidence that MpRV is not a member of the genus Aquareovirus, as members of this genus are turreted viruses.
It is interesting that, within the RdRp phylogenetic tree, the branch of MpRV dissects the tree, separating the groups of turreted and non-turreted viruses. It has been found that M. pusillla is evolutionarily older than the hosts of other members of the family Reoviridae (Bhattacharya & Medlin, 1998; Doolittle, 1999; Cavalier-Smith, 2002). The location of MpRV at the node separating the turreted and non-turreted viruses suggests that it belongs to a third branch (although non-turreted), which is possibly ancestral. The presence of an additional protein coat or a potential pseudo-envelope structure may be an ancestral character lost by other members of the family Reoviridae or a specific adaptable character of the reoviruses infecting protists.
Based on all of these findings, MpRV should be classified as a member of a novel genus within the family Reoviridae. This genus could be designated Mimoreovirus (Micromonas pusilla reovirus). A formal proposal was made to the ICTV session during the International Congress of Virology held in San Francisco, CA, USA, in July 2005 to create the genus Mimoreovirus and to designate MpRV as its type species. This proposal received initial support and was passed for wider consultation.
|
ACKNOWLEDGEMENTS |
|---|
|
REFERENCES |
|---|
|
TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONREFERENCES |
|---|
Attoui, H., Billoir, F., Cantaloube, J. F., Biagini, P., de Micco, P. & de Lamballerie, X. (2000a). Strategies for the sequence determination of viral dsRNA genomes. J Virol Methods 89, 147–158.[CrossRef][Medline]
Attoui, H., Billoir, F., Biagini, P., Cantaloube, J. F., de Chesse, R., de Micco, P. & de Lamballerie, X. (2000b). Sequence determination and analysis of the full-length genome of Colorado tick fever virus, the type species of genus Coltivirus (family Reoviridae). Biochem Biophys Res Commun 273, 1121–1125.[CrossRef][Medline]
Attoui, H., Fang, Q., Mohd Jaafar, F., Cantaloube, J.-F., Biagini, P., de Micco, P. & de Lamballerie, X. (2002a). Common evolutionary origin of aquareoviruses and orthoreoviruses revealed by genome characterization of Golden shiner reovirus, Grass carp reovirus, Striped bass reovirus and golden ide reovirus (genus Aquareovirus, family Reoviridae). J Gen Virol 83, 1941–1951.
Attoui, H., Mohd Jaafar, F., Biagini, P., Cantaloube, J.-F., de Micco, P., Murphy, F. A. & de Lamballerie, X. (2002b). Genus Coltivirus (family Reoviridae): genomic and morphologic characterization of Old World and New World viruses. Arch Virol 147, 533–561.[CrossRef][Medline]
Attoui, H., de Lamballerie, X. & Mertens, P. P. C. (2005). Coltivirus, Reoviridae. In Virus Taxonomy. Eighth Report of the International Committee on Taxonomy of Viruses, pp. 497–503. Edited by C. M. Fauquet, M. A. Mayo, J. Maniloff, U. Desselberger & L. A. Ball. London: Elsevier/Academic Press.
Baker, T. S., Olson, N. H. & Fuller, S. D. (1999). Adding the third dimension to virus life cycles: three-dimensional reconstruction of icosahedral viruses from cryo-electron micrographs. Microbiol Mol Biol Rev 63, 862–922.
Bhattacharya, D. & Medlin, L. (1998). Algal phylogeny and the origin of land plants. Plant Physiol 116, 9–15.
Brussaard, C. P. D., Noordeloos, A. A. M., Sandaa, R.-A., Heldal, M. & Bratbak, G. (2004). Discovery of a dsRNA virus infecting the marine photosynthetic protist Micromonas pusilla. Virology 319, 280–291.[CrossRef][Medline]
Burroughs, J. N., O'Hara, R. S., Smale, C. J., Hamblin, C., Walton, A., Armstrong, R. & Mertens, P. P. C. (1994). Purification and properties of virus particles, infectious subviral particles, cores and VP7 crystals of African horsesickness virus serotype 9. J Gen Virol 75, 1849–1857.
Byrd, J. C. & Bresalier, R. S. (2004). Mucins and mucin binding proteins in colorectal cancer. Cancer Metastasis Rev 23, 77–99.[CrossRef][Medline]
Cavalier-Smith, T. (2002). The phagotrophic origin of eukaryotes and phylogenetic classification of Protozoa. Int J Syst Evol Microbiol 52, 297–354.[Abstract]
Cottrell, M. T. & Suttle, C. A. (1991). Wide-spread occurrence and clonal variation in viruses which cause lysis of a cosmopolitan, eukaryotic marine phytoplankter, Micromonas pusilla. Mar Ecol Prog Ser 78, 1–9.
Diprose, J. M., Burroughs, J. N., Sutton, G. C. & 8 other authors (2001). Translocation portals for the substrates and products of a viral transcriptase complex: the bluetongue virus core. EMBO J 20, 7229–7239.[CrossRef][Medline]
Doolittle, W. F. (1999). Phylogenetic classification and the universal tree. Science 284, 2124–2128.[CrossRef][Medline]
Estes, M. K. & Cohen, J. (1989). Rotavirus gene structure and function. Microbiol Rev 53, 410–449.
Gibbs, A. & Keese, P. K. (1995). In search of the origins of viral genes. In Molecular Basis of Virus Evolution, pp. 76–90. Edited by A. Gibbs, C. H. Calisher & F. García-Arenal. Cambridge: Cambridge University Press.
Gouet, P., Diprose, J. M., Grimes, J. M., Malby, R., Burroughs, J. N., Ziéntara, S., Stuart, D. I. & Mertens, P. P. C. (1999). The highly ordered double-stranded RNA genome of bluetongue virus revealed by crystallography. Cell 97, 481–490.[CrossRef][Medline]
Grimes, J. M., Burroughs, J. N., Gouet, P., Diprose, J. M., Malby, R., Ziéntara, S., Mertens, P. P. C. & Stuart, D. I. (1998). The atomic structure of the bluetongue virus core. Nature 359, 470–478.
Harrison, P. J., Waters, R. E. & Taylor, F. J. R. (1980). A broad spectrum artificial sea water medium for coastal and open ocean phytoplankton. J Phycol 16, 28–35.[CrossRef]
Hill, C. L., Booth, T. F., Prasad, B. V. V., Grimes, J. M., Mertens, P. P. C., Sutton, G. C. & Stuart, D. I. (1999). The structure of a cypovirus and the functional organization of dsRNA viruses. Nat Struct Biol 6, 565–568.[CrossRef][Medline]
Kumar, S., Tamura, K. & Nei, M. (2004). MEGA3: integrated software for molecular evolutionary genetics analysis and sequence alignment. Brief Bioinform 5, 150–163.
Martin, L. A., Meyer, A. J., O'Hara, R. S., Fu, H., Knowles, N. J. & Mertens, P. P. C. (1998). Phylogenetic analysis of African horse sickness virus genome segment 10: sequence variation, virulence characteristics and cell exit. Arch Virol Suppl 14, 281–293.
Mertens, P. (2004). The dsRNA viruses. Virus Res 101, 3–13.[CrossRef][Medline]
Mertens, P. P. C. & Diprose, J. (2004). The bluetongue virus core: a nano-scale transcription machine. Virus Res 101, 29–43.[CrossRef][Medline]
Mertens, P. P. C., Arella, M., Attoui, H. & 41 other authors (2000). Reoviridae. In Virus Taxonomy: Seventh Report of the International Committee on Taxonomy of Viruses, pp. 395–480. Edited by M. H. V. van Regenmortel, C. M. Fauquet, D. H. L. Bishop, E. B. Carstens, M. K. Estes, S. M. Lemon, J. Maniloff, M. A. Mayo, D. J. McGeoch, C. R. Pringle & R. B. Wickner. New York, NY: Academic Press.
Mertens, P. P. C., Attoui, H., Duncan, R. & Dermody, T. S. (2005). Reoviridae. In Virus Taxonomy: Eighth Report of the International Committee on Taxonomy of Viruses, pp. 447–454. Edited by C. M. Fauquet, M. A. Mayo, J. Maniloff, U. Desselberger & L. A. Ball. London: Elsevier/Academic Press.
Mohd Jaafar, F., Attoui, H., de Micco, P. & de Lamballerie, X. (2004). Termination and read-through proteins encoded by genome segment 9 of Colorado tick fever virus. J Gen Virol 85, 2237–2244.
Mohd Jaafar, F., Attoui, H., Mertens, P., de Micco, P. & de Lamballerie, X. (2005). Structural organisation of a human encephalitic isolate of Banna virus (genus Seadornavirus, family Reoviridae). J Gen Virol 86, 1147–1157.
Murphy, F. A., Coleman, P. H., Harrison, A. K. & Gary, G. W., Jr (1968). Colorado tick fever virus: an electron microscopic study. Virology 35, 28–40.[CrossRef][Medline]
Nason, E. L., Rothagel, R., Mukherjee, S. K., Kar, A. K., Forzan, M., Prasad, B. V. & Roy, P. (2004). Interactions between the inner and outer capsids of bluetongue virus. J Virol 78, 8059–8067.
Owens, R. J., Limn, C. & Roy, P. (2004). Role of an arbovirus nonstructural protein in cellular pathogenesis and virus release. J Virol 78, 6649–6656.
Prasad, B. V. V., Wang, G. J., Clerx, J. P. M. & Chiu, W. (1988). Three-dimensional structure of rotavirus. J Mol Biol 199, 269–275.[CrossRef][Medline]
Rasmussen, S. W. (1995). DNATools, a software package for DNA sequence analysis. Carlsberg Laboratory, Copenhagen.
Reinisch, K. M., Nibert, M. L. & Harrison, S. C. (2000). Structure of the reovirus core at 3.6 Å resolution. Nature 404, 960–967.[CrossRef][Medline]
Thompson, J. D., Higgins, D. G. & Gibson, T. J. (1994). CLUSTAL W: improving the sensitivity of progressive multiple sequence alignment through sequence weighting, position-specific gap penalties and weight matrix choice. Nucleic Acids Res 22, 4673–4680.
Wommack, K. E., Ravel, J., Hill, R. T., Chun, J. & Colwell, R. R. (1999). Population dynamics of Chesapeake Bay virioplankton: total-community analysis by pulsed-field gel electrophoresis. Appl Environ Microbiol 65, 231–240.
Yeager, M., Dryden, K. A., Olson, N. H., Greenber, H. B. & Baker, T. S. (1990). Three-dimensional structure of rhesus rotavirus by cryoelectron microscopy reconstruction. J Cell Biol 110, 2133–2144.
Yeager, M., Berriman, J. A., Baker, T. A. & Bellamy, A. R. (1994). Three-dimensional structure of the rotavirus haemagglutinin VP4 by cryo-electron microscopy and difference map analysis. EMBO J 13, 1011–1018.[Medline]
Received 4 October 2005;
accepted 9 January 2006.
This article has been cited by other articles:
|
|
 |
|
  H. Mizumoto, Y. Tomaru, Y. Takao, Y. Shirai, and K. Nagasaki Diverse Responses of the Bivalve-Killing Dinoflagellate Heterocapsa circularisquama to Infection by a Single-Stranded RNA Virus Appl. Envir. Microbiol., May 15, 2008; 74(10): 3105 - 3111. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 S. Supyani, B. I. Hillman, and N. Suzuki Baculovirus expression of the 11 mycoreovirus-1 genome segments and identification of the guanylyltransferase-encoding segment J. Gen. Virol., January 1, 2007; 88(1): 342 - 350. [Abstract] [Full Text] [PDF]
|
|
| ||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||
| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
| INT J SYST EVOL MICROBIOL | MICROBIOLOGY | J GEN VIROL |
| J MED MICROBIOL | ALL SGM JOURNALS | |
