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Review

Caliciviridae Other Than Noroviruses

by
Ulrich Desselberger
Department of Medicine, University of Cambridge, Addenbrooke’s Hospital, Cambridge CB2 0QQ, UK
Viruses 2019, 11(3), 286; https://doi.org/10.3390/v11030286
Submission received: 18 January 2019 / Revised: 8 March 2019 / Accepted: 11 March 2019 / Published: 21 March 2019
(This article belongs to the Special Issue Noroviruses)
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Abstract

:
Besides noroviruses, the Caliciviridae family comprises four other accepted genera: Sapovirus, Lagovirus, Vesivirus, and Nebovirus. There are six new genera proposed: Recovirus, Valovirus, Bavovirus, Nacovirus, Minovirus, and Salovirus. All Caliciviridae have closely related genome structures, but are genetically and antigenically highly diverse and infect a wide range of mammalian host species including humans. Recombination in nature is not infrequent for most of the Caliciviridae, contributing to their diversity. Sapovirus infections cause diarrhoea in pigs, humans and other mammalian hosts. Lagovirus infections cause systemic haemorrhagic disease in rabbits and hares, and vesivirus infections lead to lung disease in cats, vesicular disease in swine, and exanthema and diseases of the reproductive system in large sea mammals. Neboviruses are an enteric pathogen of cattle, differing from bovine norovirus. At present, only a few selected caliciviruses can be propagated in cell culture (permanent cell lines or enteroids), and for most of the cultivatable caliciviruses helper virus-free, plasmid only-based reverse genetics systems have been established. The replication cycles of the caliciviruses are similar as far as they have been explored: viruses interact with a multitude of cell surface attachment factors (glycans) and co-receptors (proteins) for adsorption and penetration, use cellular membranes for the formation of replication complexes and have developed mechanisms to circumvent innate immune responses. Vaccines have been developed against lagoviruses and vesiviruses, and are under development against human noroviruses.

1. Introduction

Noroviruses (NoVs) are a major cause of epidemic acute gastroenteritis (AGE), and most chapters of this Special Issue are devoted to the structure, replication, pathogenesis, immune responses, epidemiology/evolution, and vaccine development relating to viruses of this genus of the Caliciviridae family. Murine norovirus (MuNoV) has received particular attention, since it can be propagated in cell culture [1], can be manipulated in well-developed reverse genetics systems [2,3,4,5] and has become a potent animal model of molecular-biological research [6,7,8,9]. Human noroviruses (HuNoVs) can now also be propagated in human B cells in the presence of histo-blood group antigen (HBGA) expressing bacteria or of synthetic H-type HGBA [10] or in human enteroids [11]. Reverse genetics systems for HuNoVs are under development, whereas an animal model for HuNoVs infection is in its infancy [12]. Vaccine development against human NoV disease is under intense study [13]. The present chapter aims at providing an overview on genera of the Caliciviridae family other than noroviruses*.
*The review on Caliciviridae other than noroviruses complements the many contributions to NoV research in this Special Issue of Viruses which relate to:
  • NoV structure [14];
  • The molecular biology of NoV replication [15];
  • NoV replication in the immunocompromised host [16];
  • Factors affecting host susceptibility to NoV infection [17];
  • In vitro propagation of NoVs [18];
  • Innate and acquired immune responses to NoV infections [19];
  • Molecular epidemiology of HuNoVs [20];
  • Use of animal models of NoV infection [21];
  • Treatment and development of antivirals [22];
  • Vaccine development [23].

2. Classification

The Caliciviridae family contains five genera: Norovirus, Sapovirus, Lagovirus, Vesivirus, and Nebovirus. Their taxonomy including prominent virus species is presented in Table 1. At least six additional genera, Recovirus, Valovirus, Bavovirus, Nacovirus, Minovirus and Salovirus, have been proposed (Table 1), and more may be discovered by metagenomic analyses.

3. Genome Structure

The genome organisation of the different calicivirus genera (Figure 1, reference [24]) follows the general scheme of a single-stranded, positive-sense RNA of 7.3–8.5 kb in size with a VPg covalently linked to the 5’ end and a long open reading frame (ORF) encoding a polyprotein positioned between relatively short 5’ and 3’ untranslated regions (UTR). By genome structure, the Caliciviridae can be differentiated further into two main groups. In the Norovirus, Vesivirus, and Recovirus genera ORF1 is separated from ORF2 and ORF3 near the 3’ end, and an ORF4 (comprised within ORF2) was found in MuNoV, encoding a virulence factor, VF1. The other genera (Sapovirus, Lagovirus, Nebovirus, Valovirus) possess a large ORF1 and a standard ORF2 (equivalent to ORF3 of norovirus); ORF3 (equivalent to MuNoV ORF4) has been proposed for sapovirus.

4. Replication

The replication cycle for MuNoVs has been studied in most detail [24,34]. Binding of virus to cellular attachment factors (glycans) and additional interaction with co-receptors (proteins) are followed by viral entry into the cell and release of the viral genome into the cytoplasm where it is translated. While cellular mRNAs are capped, NoV RNAs use the viral protein (VPg) which is covalently linked to the 5’ ends of both full-length genomic (g) and subgenomic (sg) RNAs, for the recruitment of cellular translation factors and ribosomes. The viral polyprotein translated from gRNA is processed by successive cleavages. Viral proteins and RNA form membrane-bound replication complexes where viral RNA replication occurs via a double-stranded RNA intermediates and where VPg-linked gRNAs and sgRNAs are produced. VP1 and VP2 are expressed from sgRNAs. Only the gRNA is then encapsidated, and particles are released by lytic or non-lytic mechanisms. The replication cycles of other members of the Caliciviridae are similar, as far as they have been studied.
Norovirus recombination appears to be a not infrequent event in nature, although it is difficult to reproduce in the laboratory [35,36].

4.1. Sapovirus

Besides NoVs, sapoviruses (SaVs) are members of the only other Calicivirus genus able to infect humans of all ages and to cause AGE, which can occur sporadically or in outbreaks. SaVs also infect pigs, mink, dogs, sea lions, and bats [37]. Like NoVs, SaVs are genomically highly diverse; so far 15 genogroups (GG) based on VP1 gene sequences have been distinguished [37,38], four of which (GGI, GGII, GGIV, and GGV) infect humans [39]. Pairwise genomic distance comparison has yielded three clearly distinct, non-overlapping peaks which represent strains, genotypes and genogroups [37] (Figure 2). (Very similar data have been obtained by pairwise genomic distance comparisons for members of many other virus families.) Within genogroups, various genotypes (GT) have been differentiated [37]. Of all genes, those encoding RdRp are most conserved. The ORFs encoding the RdRp and VP1 overlap in the so-called “junction region” which is also a hotspot for recombination [40,41]. Metagenomic identification of SaV sequences has enlarged the diversity of this genus [42]. Highly divergent sapovirus-like calicivirus genome sequences have been identified metagenomically in bats [43,44], which may play an important role in the spreading of SaVs [45].
The porcine SaV (Cowden strain) can be propagated in LLC-PK cells in the presence of intestinal content or bile acids [46], attempts to cultivate human SaVs in cell culture have so far been unsuccessful [47]. The replication cycle of the porcine SaV has been analysed in some detail. Sialic acid residues in α2.3- and α2.6-linkage act as attachment receptors for porcine SaV [48]. Porcine SaV enters cells via clathrin- and cholesterol-dependent endocytosis requiring the presence of dynamin [49]. Occludin acts as a co-receptor [50]. The cellular cap-binding protein eIF4E and RNA helicase eIF4A associate with VPg and are required for SaV translation initiation [51,52]. The PI3K/Akt and MEK/ERK signalling pathways are activated during viral entry [53]. The cyclooxygenase/prostaglandin E2 pathway is involved in SaV replication, and its blockage by specific siRNAs interferes with SaV replication [54]. A helper virus-free reverse genetics system for porcine SaV has been established [55].
SaVs of different genogroups and genotypes co-evolve in humans, preferential infection with particular genotypes, such as with HuNoV GII.4, has not been observed [37]. The overall prevalence of SaVs in low- and middle-income countries is 6.5% [56] and in high-income countries 2.2–12.7% [37].
Recently, a nucleoside acting as a viral polymerase inhibitor has been identified, which blocks the transcription of MuNoV, rotavirus, and SaV genomes in cell culture and—for rotavirus—acts as an effective antiviral in an adult mouse model [57].

4.2. Lagovirus

The genus Lagovirus contains two main species, Rabbit hemorrhagic disease virus (RHDV) and European brown hare syndrome virus (EBHSV). Due to a relatively close genomic relationship of RHDV and EBHSV, it has recently been proposed to subsume them under one species, subdivided into two genogroups (GGI, GGII) and several genotypes within genogroups [58]. Lagoviruses can cross-infect within lagomorph host species, and recombination events following dual infections are frequent [59,60,61,62,63]. Lagoviruses use host cell histo-blood group antigens (HBGA) A, B, and H (GGI) or terminal N-acetylglucosamine (GGII) as primary attachment factors [64]. After engagement with the cellular receptor, B cell epitopes on VP60, the major capsid protein, and their binding to HBGA H2 have been defined by monoclonal antibodies [65]; the binding can be blocked by immune sera of vaccinated animals [66]. Following attachment, RHDV is internalized by interaction of rabbit nucleolin with N-terminal residues of VP60 [67], and internalization can be blocked by epitope-specific peptides [67]. The viral genome-linked protein (VPg) was found to be essential for translation initiation [68]. RHDV can be propagated in vitro [69]. A reverse genetics system for Lagovirus has been described [70].
RHDV grows in multiple organs of infected animals, mainly in the liver, but also in the spleen and blood mononuclear cells, and causes disseminated intravascular coagulation, leading to multiple organ haemorrhages and necroses [71,72]. RHDV RNA has been detected in several wild small mammalian species [73]; however, no RHDV replication has been detected in mice, not even in immunodeficient animals [74]. Thus, lagovirus replication is considered to be restricted to lagomorphs as host species. Rabbits are an animal model for RHDV infection [75]. Particular RHDV strains have been demonstrated to spread rapidly within whole continents such as Australia [76]. Disease control in rabbit breeding facilities relies on biosecurity measures and vaccination [71]. Effective vaccines against RHDV infection have been produced [77,78,79,80]. On the other hand, the virus has been used with favourable outcome as biocontrol against rabbits in Australia, helped by the fact that the virus was not transmitted to non-target host species [81]. RHDV-related non-pathogenic rabbit calicivirus (RCV) strains are endemic in New Zealand and Australia, and there is evidence that prior exposure of rabbits to RCV reduces the frequency of and mortality from RHDV infection [82,83].

4.3. Vesivirus

Feline calicivirus (FCV) is the major representative of this Calicivirus genus, causing mainly upper and rarely lower respiratory tract diseases. Some virulent strains cause systemic disease, including subcutaneous oedema, necroses in multiple organs (liver, spleen, pancreas) and interstitial pneumonia [84,85]. Until recently, it was the first and only calicivirus which could be propagated in various cell lines, such as Vero cells, BHK cells, 293 cells [86], and also in feline mammary epithelial cells [87]. Other vesiviruses are Vesicular exanthema of swine virus, which causes vesicular disease and foetal damage in swine [88,89], and the San Miguel sea lion virus, which produces exanthemas and diseases of the reproductive system in large sea mammals [90,91].
FCV enters cells by first binding to α2,6-linked sialic acid as an attachment receptor and then interacts with the feline junctional adhesion molecular A (fJAM-A), which serves as a functional co-receptor [86,92]. Recently it has been demonstrated that upon the interaction of FCV particles with a soluble fJAM A fragment, 12 molecules of the minor capsid protein VP2 form large portal entry-like assemblies at a three-fold axis of symmetry, with the hydrophobic N-termini of VP2 pointing away from the viral surface. This leads to the opening of a pore in the capsid shell through which the viral genome may be delivered into the cytoplasm of a host cell [93]. Since all caliciviruses encode a VP2, these morphological changes upon viral entry may be a general phenomenon [93].
Due to its longstanding cultivability, there is more detailed information on the FCV replication cycle. Conserved amino acid residues in the capsid protein of FCV were identified which were essential for interaction with fJAM-A [94]. Knockdown of nucleolin (NCL), a phosphoprotein involved in ribosome biogenesis, was shown to reduce FCV protein synthesis and the yield of viral progeny; but the binding of NCL to both ends of the FCV RNA stimulated its translation [95]. Inactivation of NCL by the aptamer AGRO100 could be reversed by NCL overexpression [95]. Infection of cells with FCV led to activation of the COX-2 PGE2 pathway, which promotes viral replication [96]. siRNA-induced inhibition of COX-2 blocked viral replication, but this could be restored by the addition of PGE2 [96]. One of the non-structural proteins of FCV, p39, was shown to suppress IFN type I production by preventing IRF-3 activation [97]. FCV-infected cells did not produce stress granules (SG), since the viral protease (encoded by ORF NS6) cleaved one of the SG-activating proteins [98]. Host gene expression at the transcriptional level was prevented (“shut off”) by FCV-encoded protease-polymerase protein [99]. Several plasmid only-based reverse genetics systems were developed for FCV [100,101]. Although FCV genomes were found to vary extensively in a European surveillance study, antibodies raised against an FCV isolate obtained more than five decades ago broadly cross-reacted with and cross-neutralized contemporary FCV strains [102]. Cats are a natural model for FCV infection [103]. FCV vaccines were developed more than 10 years ago [104]. Recent FCV vaccine-induced antibodies were found to be of considerable cross-NT activity, in particular when dual vaccine preparations were used [105]. Intranasal immunization with inactivated FCV particles was found to be particularly effective in conveying robust protection [106].
Vesiviruses have also been recognized as infectious agents for household dogs in Italy [107] and more recently in association with an outbreak of acute haemorrhagic gastroenteritis in dogs in the USA [108]. The canine caliciviruses (CCaV) were found to be related to so-called 2117-like vesiviruses originally discovered as contaminants of Chinese hamster ovary cells [109]. Since CCaVs cross-react with the sera of cats, cross-infection of dogs with FCV or possibly infection of cats with 2117-like viruses were suggested [109]. Vesivirus 2117 is able to infect various cell lines [110]. Interestingly, morphologically the capsids of 2117-like vesiviruses more closely resemble sapovirus- and lagovirus-like particles than those of other vesiviruses [111].
The Hom-1 calicivirus, isolated from a human laboratory worker in 1998 as an inadvertent transmission of the San Miguel sea lion virus [90], was found to use the human JAM-1 (hJAM-1) molecule as its receptor in HepG2, HuH7 and SK-CO15 cells [112].
Some authors have suggested that vesivirus infection in humans may be quite common and possibly be associated with hepatitis of unknown but suspected infectious cause [113,114].

4.4. Nebovirus

In 2006 the sequence of a cattle-pathogenic enteric virus, Newbury agent-1, was determined and proposed as a new genus, Nebovirus, of the Caliciviridae [115]. Nebovirus interacts with a wide spectrum of HBGAs [116]. Recombination in different regions of the nebovirus genome was observed [117,118], similar to that in other genera of the Caliciviridae. Infection of calves with bovine NoV and nebovirus appears to be common in the USA [119], Brazil [120], Turkey [121], Iran [122], Korea [123], and China [124,125].

4.5. Recovirus

A rhesus macaque was the source of a novel calicivirus, named Tulane Virus (TV), which although most closely related to NoVs, was sufficiently different in nucleotide sequence from other caliciviruses to justify classification in a new genus, Recovirus [126]. Recoviruses have considerable genomic and antigenic diversity [127], and different genogroups and genotypes can be distinguished, similar to the HuNoV classification [127]. Tulane virus grows in monkey kidney cells and relies on HBGAs as a primary attachment factor [128,129,130]. A reverse genetics system for Tulane virus has been established [131]. Biologically, Tulane virus behaves similar to human NoVs, such as being shed in feces in large quantities and being transmitted by the fecal-oral route, and it has been proposed as a surrogate model for human NoV AGE [132]. Recovirus infection elicits RIG-I- and MDA-5-dependent innate immune responses at different stages of recovirus replication [133]. Recovirus-like viruses were found in the feces of Amerindian children in isolated villages of the Amazonian region of Brazil [134], and recovirus-specific neutralizing antibodies were observed in zookeepers who were in contact with monkeys [135]. A recovirus-related virus, which however had human NoV-like capsid sequences, was recently isolated from bats [136].

4.6. Valovirus

Between 2005 and 2007, caliciviruses isolated from pigs in Canada were proposed as a new genus, Valovirus [25] (Figure 3). Similar viruses were detected in pigs in Italy in 2010 [26,27] and more recently isolated from bats in Hungary [43].

4.7. Bavovirus and Nacovirus

Between 2009 and 2011 caliciviruses were isolated from chicken and turkey from German farms. Phylogenetic analysis of partial deduced amino acid sequences of the non-structural protease and polymerase genes (320–350 aa) and of the VP1 gene (530–700 aa) strongly suggested the presence of new genera, and the names Bavovirus (chicken) and Nacovirus (turkey) were proposed [28]. Of 24 chicken farms tested, 83% were positive for bavovirus, 46% were positive for nacovirus, and 38% were positive for both [28]. A naco-like virus was also isolated from a goose [29] (Figure 4).

4.8. Salovirus and Minovirus

Novel caliciviruses have been isolated from fish and have been proposed as new genera: Salovirus (from Atlantic salmon) and Minovirus (from bitterfish) [30,31].

5. Concluding Remarks

Major progress in calicivirus research has been made by the availability of a combination of tools:
  • The ability to propagate viruses in cell/enteroid culture;
  • The availability of helper virus-free (plasmid only-based) reverse genetics systems;
  • The availability of suitable animal models.
These tools have been achieved for MuNoV and are close to being fulfilled for HuNoVs. The degree to which these pre-conditions have been accomplished for the other genera of the Caliciviridae is summarized in Table 2. Progress is considered to be very advanced for the genera Lagovirus and Vesivirus, with the other genera requiring further investigation. Recombination in nature has been documented for Sapovirus, Lagovirus, and Nebovirus, and thus seems to be a general feature of the caliciviruses. Since many genera of the Caliciviridae contain important human and animal pathogens, future research will be driven by scientific curiosity as well as public health and economic needs.

Funding

This research received no external funding.

Acknowledgments

The author gratefully acknowledges the comments of Jacques LePendu and Kyoung-Oh Cho on an early version of the manuscript.

Conflicts of Interest

The author declares no conflict of interest.

References

  1. Wobus, C.E.; Karst, S.M.; Thackray, L.B.; Chang, K.O.; Sosnovtsev, S.V.; Belliot, G.; Krug, A.; Mackenzie, J.M.; Green, K.Y.; Virgin, H.W. Replication of Norovirus in cell culture reveals a tropism for dendritic cells and macrophages. PLoS Biol. 2004, 2, e432. [Google Scholar] [CrossRef]
  2. Ward, V.K.; McCormick, C.J.; Clarke, I.N.; Salim, O.; Wobus, C.E.; Thackray, L.B.; Virgin, H.W., 4th; Lambden, P.R. Recovery of infectious murine norovirus using pol II-driven expression of full-length cDNA. Proc. Natl. Acad. Sci. USA 2007, 104, 11050–11055. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  3. Chaudhry, Y.; Skinner, M.A.; Goodfellow, I.G. Recovery of genetically defined murine norovirus in tissue culture by using a fowlpox virus expressing T7 RNA polymerase. J Gen Virol. 2007, 88 Pt 8, 2091–2100. [Google Scholar] [CrossRef] [Green Version]
  4. Yunus, M.A.; Chung, L.M.; Chaudhry, Y.; Bailey, D.; Goodfellow, I. Development of an optimized RNA-based murine norovirus reverse genetics system. J. Virol. Methods 2010, 169, 112–118. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  5. Arias, A.; Bailey, D.; Chaudhry, Y.; Goodfellow, I. Development of a reverse-genetics system for murine norovirus 3: Long-term persistence occurs in the caecum and colon. J. Gen. Virol. 2012, 93 Pt 7, 1432–1441. [Google Scholar] [CrossRef]
  6. Nice, T.J.; Strong, D.W.; McCune, B.T.; Pohl, C.S.; Virgin, H.W. A single-amino-acid change in murine norovirus NS1/2 is sufficient for colonic tropism and persistence. J. Virol. 2013, 87, 327–334. [Google Scholar] [CrossRef] [PubMed]
  7. Ohsugi, T.; Matsuura, K.; Kawabe, S.; Nakamura, N.; Kumar, J.M.; Wakamiya, M.; Morikawa, S.; Urano, T. Natural infection of murine norovirus in conventional and specific pathogen-free laboratory mice. Front. Microbiol. 2013, 4, 12. [Google Scholar] [CrossRef] [PubMed]
  8. Kolawole, A.O.; Gonzalez-Hernandez, M.B.; Turula, H.; Yu, C.; Elftman, M.D.; Wobus, C.E. Oral norovirus infection is blocked in mice lacking Peyer’s patches and mature M cells. J. Virol. 2015, 90, 1499–1506. [Google Scholar] [CrossRef] [PubMed]
  9. Kolawole, A.O.; Rocha-Pereira, J.; Elftman, M.D.; Neyts, J.; Wobus, C.E. Inhibition of human norovirus by a viral polymerase inhibitor in the B cell culture system and in the mouse model. Antivir. Res. 2016, 132, 46–49. [Google Scholar] [CrossRef] [Green Version]
  10. Jones, M.K.; Watanabe, M.; Zhu, S.; Graves, C.L.; Keyes, L.R.; Grau, K.R.; Gonzalez-Hernandez, M.B.; Iovine, N.M.; Wobus, C.E.; Vinjé, J.; et al. Enteric bacteria promote human and mouse norovirus infection of B cells. Science 2014, 346, 755–759. [Google Scholar] [CrossRef] [Green Version]
  11. Ettayebi, K.; Crawford, S.E.; Murakami, K.; Broughman, J.R.; Karandikar, U.; Tenge, V.R.; Neill, F.H.; Blutt, S.E.; Zeng, X.L.; Qu, L.; et al. Replication of human noroviruses in stem cell-derived human enteroids. Science 2016, 353, 1387–1393. [Google Scholar] [CrossRef]
  12. Taube, S.; Kolawole, A.O.; Höhne, M.; Wilkinson, J.E.; Handley, S.A.; Perry, J.W.; Thackray, L.B.; Akkina, R.; Wobus, C.E. A mouse model for human norovirus. MBio 2013, 4, e00450. [Google Scholar] [CrossRef]
  13. Cortes-Penfield, N.W.; Ramani, S.; Estes, M.K.; Atmar, R.L. Prospects and challenges in the development of a norovirus vaccine. Clin. Ther. 2017, 39, 1537–1549. [Google Scholar] [CrossRef]
  14. Smith, H.Q.; Smith, T.J. The Dynamic Capsid Structures of the Noroviruses. Viruses 2019, 11, 235. [Google Scholar] [CrossRef]
  15. Goodfellow, I.; Vinje, J.; Wilen, C.; Mackenzie, J.; White, P.; Karst, S.; Taube, S.; Hwang, S.; Ward, V. The molecular biology of NoV replication. Viruses, in preparation.
  16. Debbink, K.; Chong, P. NoV replication in the immunocompromised host. Viruses, in preparation.
  17. Nordgren, J.; Svensson, L. Genetic Susceptibility to Human Norovirus Infection: An Update. Viruses 2019, 11, 226. [Google Scholar] [CrossRef]
  18. Jones, M.; Estes, M.K. In vitro propagation of NoVs. Viruses, in preparation.
  19. Baric, R.; Lindesmith, L.; Mallory, M.; Brewer-Jensen, P. Innate and acquired immune responses to NoV infections. Viruses, in preparation.
  20. Schultz-Cherry, S.; Mans, J.; Moe, C.; Kirby, A.; Teunis, P.; Lopman, B.A.; Hall, A.J.; Guix, S.; Blazevic, V.; Andrade, J.S.R. Molecular epidemiology of HuNoVs. Viruses, in preparation.
  21. Todd, K.V.; Tripp, R.A. Human Norovirus: Experimental Models of Infection. Viruses 2019, 11, 151. [Google Scholar] [CrossRef]
  22. Chang, K.O.; Kim, Y.; Lovell, S.; Rathnayake, A.D.; Groutas, W.C. Antiviral Drug Discovery: Norovirus Proteases and Development of Inhibitors. Viruses 2019, 11, 197. [Google Scholar] [CrossRef]
  23. Brown, R. Vaccine development. Viruses, in preparation.
  24. Goodfellow, I.; Taube, S. Calicivirus replication and reverse genetics. In Viral Gastroenteritis; Svensson, L., Desselberger, U., Greenberg, H.B., Estes, M.K., Eds.; Elsevier Academic Press: Amsterdam, The Netherlands, 2016; pp. 355–378. [Google Scholar]
  25. L’Homme, Y.; Sansregret, R.; Plante-Fortier, E.; Lamontagne, A.M.; Ouardani, M.; Lacroix, G.; Simard, C. Genomic characterization of swine caliciviruses representing a new genus of Caliciviridae. Virus Genes 2009, 39, 66–75. [Google Scholar] [CrossRef]
  26. Di Martino, B.; Martella, V.; Di Profio, F.; Ceci, C.; Marsilio, F. Detection of St-Valerien-like viruses in swine, Italy. Vet. Microbiol. 2011, 149, 221–224. [Google Scholar] [CrossRef]
  27. Di Martino, B.; Di Profio, F.; Ceci, C.; Martella, V.; Lavazza, A.; Massirio, I.; Marsilio, F. Seroprevalence of St-Valerien-like caliciviruses in Italian swine. J. Gen. Virol. 2012, 93 Pt 1, 102–105. [Google Scholar] [CrossRef]
  28. Wolf, S.; Reetz, J.; Hoffmann, K.; Gründel, A.; Schwarz, B.A.; Hänel, I.; Otto, P.H. Discovery and genetic characterization of novel caliciviruses in German and Dutch poultry. Arch. Virol. 2012, 157, 1499–1507. [Google Scholar] [CrossRef] [PubMed]
  29. Liao, Q.; Wang, X.; Wang, D.; Zhang, D. Complete genome sequence of a novel calicivirus from a goose. Arch. Virol. 2014, 159, 2529–2531. [Google Scholar] [CrossRef] [PubMed]
  30. Mikalsen, A.B.; Nilsen, P.; Frøystad-Saugen, M.; Lindmo, K.; Eliassen, T.M. Characterization of a novel calicivirus causing systemic infection in atlantic salmon (Salmo salar L.): Proposal for a new genus of Caliciviridae. PLoS ONE 2014, 9, e107132. [Google Scholar] [CrossRef] [PubMed]
  31. Mor, S.K.; Phelps, N.B.D.; Ng, T.F.F.; Subramaniam, K.; Primus, A.; Armien, A.G.; McCann, R.; Puzach, C.; Waltzek, T.B.; Goyal, S.M. Genomic characterization of a novel calicivirus, FHMCV-2012, from baitfish in the USA. Arch. Virol. 2017, 162, 3619–3627. [Google Scholar] [CrossRef]
  32. McCune, B.T.; Tang, W.; Lu, J.; Eaglesham, J.B.; Thorne, L.; Mayer, A.E.; Condiff, E.; Nice, T.J.; Goodfellow, I.; Krezel, A.M.; et al. Noroviruses co-opt the function of host proteins VAPA and VAPB for replication via a phenylalanine-phenylalanine-acidic-tract-motif mimic in nonstructural viral protein NS1/2. MBio 2017, 8, e00668-17. [Google Scholar] [CrossRef] [PubMed]
  33. Doerflinger, S.Y.; Cortese, M.; Romero-Brey, I.; Menne, Z.; Tubiana, T.; Schenk, C.; White, P.A.; Bartenschlager, R.; Bressanelli, S.; Hansman, G.S.; et al. Membrane alterations induced by nonstructural proteins of human norovirus. PLoS Pathog. 2017, 13, e1006705. [Google Scholar] [CrossRef]
  34. Thorne, L.G.; Goodfellow, I.G. Norovirus gene expression and replication. J. Gen. Virol. 2014, 95 Pt 2, 278–291. [Google Scholar] [CrossRef]
  35. Bull, R.A.; Tanaka, M.M.; White, P.A. Norovirus recombination. J. Gen. Virol. 2007, 88, 3347–3359. [Google Scholar] [CrossRef] [Green Version]
  36. Ludwig-Begall, L.F.; Mauroy, A.; Thiry, E. Norovirus recombinants: Recurrent in the field, recalcitrant in the lab—A scoping review of recombination and recombinant types of noroviruses. J. Gen. Virol. 2018, 99, 970–988. [Google Scholar] [CrossRef]
  37. Oka, T.; Wang, Q.; Katayama, K.; Saif, L.J. Comprehensive review of human sapoviruses. Clin. Microbiol. Rev. 2015, 28, 32–53. [Google Scholar] [CrossRef]
  38. Oka, T.; Lu, Z.; Phan, T.; Delwart, E.L.; Saif, L.J.; Wang, Q. Genetic characterization and classification of human and animal sapoviruses. PLoS ONE 2016, 11, e0156373. [Google Scholar] [CrossRef] [PubMed]
  39. Kumthip, K.; Khamrin, P.; Maneekarn, N. Molecular epidemiology and genotype distributions of noroviruses and sapoviruses in Thailand 2000-2016: A review. J. Med. Virol. 2018, 90, 617–624. [Google Scholar] [CrossRef]
  40. Kuroda, M.; Masuda, T.; Ito, M.; Naoi, Y.; Doan, Y.H.; Haga, K.; Tsuchiaka, S.; Kishimoto, M.; Sano, K.; Omatsu, T.; et al. Genetic diversity and intergenogroup recombination events of sapoviruses detected from feces of pigs in Japan. Infect. Genet. Evol. 2017, 55, 209–217. [Google Scholar] [CrossRef] [PubMed]
  41. Diez-Valcarce, M.; Castro, C.J.; Marine, R.L.; Halasa, N.; Mayta, H.; Saito, M.; Tsaknaridis, L.; Pan, C.Y.; Bucardo, F.; Becker-Dreps, S.; et al. Genetic diversity of human sapovirus across the Americas. J. Clin. Virol. 2018, 104, 65–72. [Google Scholar] [CrossRef]
  42. Li, J.; Zhang, W.; Cui, L.; Shen, Q.; Hua, X. Metagenomic identification, genetic characterization and genotyping of porcine sapoviruses. Infect. Genet. Evol. 2018, 62, 244–252. [Google Scholar] [CrossRef] [PubMed]
  43. Kemenesi, G.; Gellért, Á.; Dallos, B.; Görföl, T.; Boldogh, S.; Estók, P.; Marton, S.; Oldal, M.; Martella, V.; Bányai, K.; et al. Sequencing and molecular modeling identifies candidate members of Caliciviridae family in bats. Infect. Genet. Evol. 2016, 41, 227–232. [Google Scholar] [CrossRef] [PubMed]
  44. Yinda, C.K.; Conceição-Neto, N.; Zeller, M.; Heylen, E.; Maes, P.; Ghogomu, S.M.; Van Ranst, M.; Matthijnssens, J. Novel highly divergent sapoviruses detected by metagenomics analysis in straw-colored fruit bats in Cameroon. Emerg. Microbes Infect. 2017, 6, e38. [Google Scholar] [CrossRef]
  45. Barry, A.F.; Durães-Carvalho, R.; Oliveira-Filho, E.F.; Alfieri, A.A.; Van der Poel, W.H.M. High-resolution phylogeny providing insights towards the epidemiology, zoonotic aspects and taxonomy of sapoviruses. Infect. Genet. Evol. 2017, 56, 8–13. [Google Scholar] [CrossRef] [PubMed]
  46. Lu, Z.; Yokoyama, M.; Chen, N.; Oka, T.; Jung, K.; Chang, K.O.; Annamalai, T.; Wang, Q.; Saif, L.J. Mechanism of cell culture adaptation of an enteric calicivirus, the porcine sapovirus Cowden Strain. J. Virol. 2015, 90, 1345–1358. [Google Scholar] [CrossRef] [PubMed]
  47. Oka, T.; Stoltzfus, G.T.; Zhu, C.; Jung, K.; Wang, Q.; Saif, L.J. Attempts to grow human noroviruses, a sapovirus, and a bovine norovirus in vitro. PLoS ONE 2018, 13, e0178157. [Google Scholar] [CrossRef]
  48. Kim, D.S.; Hosmillo, M.; Alfajaro, M.M.; Kim, J.Y.; Park, J.G.; Son, K.Y.; Ryu, E.H.; Sorgeloos, F.; Kwon, H.J.; Park, S.J.; et al. Both α2,3- and α2,6-linked sialic acids on O-linked glycoproteins act as functional receptors for porcine Sapovirus. PLoS Pathog. 2014, 10, e1004172. [Google Scholar] [CrossRef] [PubMed]
  49. Soliman, M.; Kim, D.S.; Kim, C.; Seo, J.Y.; Kim, J.Y.; Park, J.G.; Alfajaro, M.M.; Baek, Y.B.; Cho, E.H.; Park, S.I.; et al. Porcine sapovirus Cowden strain enters LLC-PK cells via clathrin- and cholesterol-dependent endocytosis with the requirement of dynamin II. Vet. Res. 2018, 49, 92. [Google Scholar] [CrossRef]
  50. Alfajaro, M.M.; Cho, E.H.; Kim, D.S.; Kim, J.Y.; Park, J.G.; Soliman, M.; Baek, Y.B.; Park, C.H.; Kang, M.I.; Park, S.I.; et al. Early infection of porcine sapovirus disrupts tight junction and uses occludin as a co-receptor. J. Virol. 2018, JVI.01773-18. [Google Scholar] [CrossRef] [PubMed]
  51. Hosmillo, M.; Chaudhry, Y.; Kim, D.S.; Goodfellow, I.; Cho, K.O. Sapovirus translation requires an interaction between VPg and the cap binding protein eIF4E. J. Virol. 2014, 88, 12213–12221. [Google Scholar] [CrossRef] [PubMed]
  52. Hosmillo, M.; Sweeney, T.R.; Chaudhry, Y.; Leen, E.; Curry, S.; Goodfellow, I.; Cho, K.O. The RNA helicase eIF4A is required for sapovirus translation. J. Virol. 2016, 90, 5200–5204. [Google Scholar] [CrossRef] [PubMed]
  53. Soliman, M.; Kim, D.S.; Park, J.G.; Kim, J.Y.; Alfajaro, M.M.; Baek, Y.B.; Cho, E.H.; Park, C.H.; Kang, M.I.; Park, S.I.; et al. PI3K/Akt and MEK/ERK signaling pathways facilitate sapovirus trafficking and late endosomal acidification for viral uncoating in LLC-PK cells. J. Virol. 2018, 92, JVI.01674-18. [Google Scholar] [CrossRef]
  54. Alfajaro, M.M.; Choi, J.S.; Kim, D.S.; Seo, J.Y.; Kim, J.Y.; Park, J.G.; Soliman, M.; Baek, Y.B.; Cho, E.H.; Kwon, J.; et al. Activation of COX-2/PGE2 promotes sapovirus replication via the inhibition of nitric oxide production. J. Virol. 2017, 91, e01656-16. [Google Scholar] [CrossRef]
  55. Chang, K.O.; Sosnovtsev, S.V.; Belliot, G.; Wang, Q.; Saif, L.J.; Green, K.Y. Reverse genetics system for porcine enteric calicivirus, a prototype sapovirus in the Caliciviridae. J. Virol. 2005, 79, 1409–1416. [Google Scholar] [CrossRef]
  56. Magwalivha, M.; Kabue, J.P.; Traore, A.N.; Potgieter, N. Prevalence of human sapovirus in low and middle income countries. Adv. Virol. 2018, 2018, 5986549. [Google Scholar] [CrossRef]
  57. Van Dycke, J.; Arnoldi, F.; Papa, G.; Vandepoele, J.; Burrone, O.R.; Mastrangelo, E.; Tarantino, D.; Heylen, E.; Neyts, J.; Rocha-Pereira, J. A single nucleoside viral polymerase inhibitor against norovirus, rotavirus, and sapovirus-induced diarrhea. J. Infect. Dis. 2018, 218, 1753–1758. [Google Scholar] [CrossRef]
  58. Le Pendu, J.; Abrantes, J.; Bertagnoli, S.; Guitton, J.S.; Le Gall-Reculé, G.; Lopes, A.M.; Marchandeau, S.; Alda, F.; Almeida, T.; Célio, A.P.; et al. Proposal for a unified classification system and nomenclature of lagoviruses. J. Gen. Virol. 2017, 98, 1658–1666. [Google Scholar] [CrossRef]
  59. Lopes, A.M.; Dalton, K.P.; Magalhães, M.J.; Parra, F.; Esteves, P.J.; Holmes, E.C.; Abrantes, J. Full genomic analysis of new variant rabbit hemorrhagic disease virus revealed multiple recombination events. J. Gen. Virol. 2015, 96 Pt 6, 1309–1319. [Google Scholar] [CrossRef]
  60. Hu, B.; Wang, F.; Fan, Z.; Song, Y.; Abrantes, J.; Zuo, Y.; Esteves, P.J. Recombination between G2 and G6 strains of rabbit hemorrhagic disease virus (RHDV) in China. Arch. Virol. 2017, 162, 269–272. [Google Scholar] [CrossRef]
  61. Silvério, D.; Lopes, A.M.; Melo-Ferreira, J.; Magalhães, M.J.; Monterroso, P.; Serronha, A.; Maio, E.; Alves, P.C.; Esteves, P.J.; Abrantes, J. Insights into the evolution of the new variant rabbit haemorrhagic disease virus (GI.2) and the identification of novel recombinant strains. Transbound. Emerg. Dis. 2018, 65, 983–992. [Google Scholar] [CrossRef]
  62. Hall, R.N.; Mahar, J.E.; Read, A.J.; Mourant, R.; Piper, M.; Huang, N.; Strive, T. A strain-specific multiplex RT-PCR for Australian rabbit haemorrhagic disease viruses uncovers a new recombinant virus variant in rabbits and hares. Transbound. Emerg. Dis. 2018, 65, e444–e456. [Google Scholar] [CrossRef]
  63. Lopes, A.M.; Rouco, C.; Esteves, P.J.; Abrantes, J. GI.1b/GI.1b/GI.2 recombinant rabbit hemorrhagic disease virus 2 (Lagovirus europaeus/GI.2) in Morocco, Africa. Arch. Virol. 2019, 164, 279–283. [Google Scholar] [CrossRef]
  64. Lopes, A.M.; Breiman, A.; Lora, M.; Le Moullac-Vaidye, B.; Galanina, O.; Nyström, K.; Marchandeau, S.; Le Gall-Reculé, G.; Strive, T.; Neimanis, A.; et al. Host specific glycans are correlated with susceptibility to infection by lagoviruses, but not with their virulence. J. Virol. 2018, 92, e01759-17. [Google Scholar] [CrossRef]
  65. Song, Y.; Wang, F.; Fan, Z.; Hu, B.; Liu, X.; Wei, H.; Xue, J.; Xu, W.; Qiu, R. Identification of novel rabbit hemorrhagic disease virus B-cell epitopes and their interaction with host histo-blood group antigens. J. Gen. Virol. 2016, 97, 356–365. [Google Scholar] [CrossRef] [Green Version]
  66. Song, Y.; Fan, Z.; Zuo, Y.; Wei, H.; Hu, B.; Chen, M.; Qiu, R.; Xue, J.; Wang, F. Binding of rabbit hemorrhagic disease virus-like particles to host histo-blood group antigens is blocked by antisera from experimentally vaccinated rabbits. Arch. Virol. 2017, 162, 3425–3430. [Google Scholar] [CrossRef]
  67. Zhu, J.; Miao, Q.; Tang, J.; Wang, X.; Dong, D.; Liu, T.; Qi, R.; Yang, Z.; Liu, G. Nucleolin mediates the internalization of rabbit hemorrhagic disease virus through clathrin-dependent endocytosis. PLoS Pathog. 2018, 14, e1007383. [Google Scholar] [CrossRef]
  68. Zhu, J.; Wang, B.; Miao, Q.; Tan, Y.; Li, C.; Chen, Z.; Guo, H.; Liu, G. Viral genome-linked protein (VPg) is essential for translation initiation of rabbit hemorrhagic disease virus (RHDV). PLoS ONE 2015, 10, e0143467. [Google Scholar] [CrossRef] [PubMed]
  69. Zhu, J.; Miao, Q.; Tan, Y.; Guo, H.; Liu, T.; Wang, B.; Chen, Z.; Li, C.; Liu, G. Inclusion of an Arg-Gly-Asp receptor-recognition motif into the capsid protein of rabbit hemorrhagic disease virus enables culture of the virus in vitro. J. Biol. Chem. 2017, 292, 8605–8615. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  70. Liu, G.; Ni, Z.; Yun, T.; Yu, B.; Chen, L.; Zhao, W.; Hua, J.; Chen, J. A DNA-launched reverse genetics system for rabbit hemorrhagic disease virus reveals that the VP2 protein is not essential for virus infectivity. J. Gen. Virol. 2008, 89 Pt 12, 3080–3085. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  71. Abrantes, J.; van der Loo, W.; Le Pendu, J.; Esteves, P.J. Rabbit haemorrhagic disease (RHD) and rabbit haemorrhagic disease virus (RHDV): A review. Vet. Res. 2012, 43, 12. [Google Scholar] [CrossRef] [PubMed]
  72. Neimanis, A.; Larsson Pettersson, U.; Huang, N.; Gavier-Widén, D.; Strive, T. Elucidation of the pathology and tissue distribution of Lagovirus europaeus GI.2/RHDV2 (rabbit haemorrhagic disease virus 2) in young and adult rabbits (Oryctolagus cuniculus). Vet. Res. 2018, 49, 46. [Google Scholar] [CrossRef] [PubMed]
  73. Rocha, G.; Alda, F.; Pagés, A.; Merchán, T. Experimental transmission of rabbit haemorrhagic disease virus (RHDV) from rabbit to wild mice (Mus spretus and Apodemus sylvaticus) under laboratory conditions. Infect. Genet. Evol. 2017, 47, 94–98. [Google Scholar] [CrossRef]
  74. Urakova, N.; Hall, R.; Strive, T.; Frese, M. Restricted host specificity of Rabbit Hemorrhagic Disease Virus is supported by challenge experiments in immune-compromised mice (Mus musculus). J. Wildl. Dis. 2019, 55, 218–222. [Google Scholar] [CrossRef]
  75. Henning, J.; Meers, J.; Davies, P.R. Exposure of rabbits to ultraviolet light-inactivated rabbit haemorrhagic disease virus (RHDV) and subsequent challenge with virulent virus. Epidemiol. Infect. 2005, 133, 731–735. [Google Scholar] [CrossRef] [Green Version]
  76. Mahar, J.E.; Hall, R.N.; Peacock, D.; Kovaliski, J.; Piper, M.; Mourant, R.; Huang, N.; Campbell, S.; Gu, X.; Read, A.; et al. Rabbit haemorrhagic disease virus 2 (GI.2) is replacing endemic strains of RHDV in the Australian landscape within 18 months of its arrival. J. Virol. 2018, 92, e01374-17. [Google Scholar]
  77. Laurent, S.; Vautherot, J.F.; Madelaine, M.F.; Le Gall, G.; Rasschaert, D. Recombinant rabbit hemorrhagic disease virus capsid protein expressed in baculovirus self-assembles into viruslike particles and induces protection. J. Virol. 1994, 68, 6794–6798. [Google Scholar]
  78. Marín, M.S.; Martín Alonso, J.M.; Pérez Ordoyo García, L.I.; Boga, J.A.; Argüello-Villares, J.L.; Casais, R.; Venugopal, K.; Jiang, W.; Gould, E.A.; Parra, F. Immunogenic properties of rabbit haemorrhagic disease virus structural protein VP60 expressed by a recombinant baculovirus: An efficient vaccine. Virus Res. 1995, 39, 119–128. [Google Scholar] [CrossRef]
  79. Boga, J.A.; Martín Alonso, J.M.; Casais, R.; Parra, F. A single dose immunization with rabbit haemorrhagic disease virus major capsid protein produced in Saccharomyces cerevisiae induces protection. J. Gen. Virol. 1997, 78 Pt 9, 2315–2318. [Google Scholar] [CrossRef] [PubMed]
  80. Castañón, S.; Marín, M.S.; Martín-Alonso, J.M.; Boga, J.A.; Casais, R.; Humara, J.M.; Ordás, R.J.; Parra, F. Immunization with potato plants expressing VP60 protein protects against rabbit hemorrhagic disease virus. J. Virol. 1999, 73, 4452–4455. [Google Scholar]
  81. Di Giallonardo, F.; Holmes, E.C. Viral biocontrol: Grand experiments in disease emergence and evolution. Trends Microbiol. 2015, 23, 83–90. [Google Scholar] [CrossRef] [PubMed]
  82. Nicholson, L.J.; Mahar, J.E.; Strive, T.; Zheng, T.; Holmes, E.C.; Ward, V.K.; Duckworth, J.A. Benign rabbit calicivirus in New Zealand. Appl. Environ. Microbiol. 2017, 83, e00090-17. [Google Scholar] [CrossRef]
  83. Cooke, B.D.; Duncan, R.P.; McDonald, I.; Liu, J.; Capucci, L.; Mutze, G.J.; Strive, T. Prior exposure to non-pathogenic calicivirus RCV-A1 reduces both infection rate and mortality from rabbit haemorrhagic disease in a population of wild rabbits in Australia. Transbound. Emerg. Dis. 2018, 65, e470–e477. [Google Scholar] [CrossRef]
  84. Pedersen, N.C.; Elliott, J.B.; Glasgow, A.; Poland, A.; Keel, K. An isolated epizootic of hemorrhagic-like fever in cats caused by a novel and highly virulent strain of feline calicivirus. Vet. Microbiol. 2000, 73, 281–300. [Google Scholar] [CrossRef]
  85. Radford, A.D.; Coyne, K.P.; Dawson, S.; Porter, C.J.; Gaskell, R.M. Feline calicivirus. Vet. Res. 2007, 38, 319–335. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  86. Makino, A.; Shimojima, M.; Miyazawa, T.; Kato, K.; Tohya, Y.; Akashi, H. Junctional adhesion molecule 1 is a functional receptor for feline calicivirus. J. Virol. 2016, 80, 4482–4490. [Google Scholar] [CrossRef]
  87. Pesavento, P.; Liu, H.; Ossiboff, R.J.; Stucker, K.M.; Heymer, A.; Millon, L.; Wood, J.; van der List, D.; Parker, J.S. Characterization of a continuous feline mammary epithelial cell line susceptible to feline epitheliotropic viruses. J. Virol. Methods 2009, 157, 105–110. [Google Scholar] [CrossRef] [PubMed]
  88. Edwards, J.F.; Yedloutschnig, R.J.; Dardiri, A.H.; Callis, J.J. Vesicular exanthema of swine virus: Isolation and serotyping of field samples. Can. J. Vet. Res. 1987, 51, 358–362. [Google Scholar]
  89. Neill, J.D.; Meyer, R.F.; Seal, B.S. The capsid protein of vesicular exanthema of swine virus serotype A48: Relationship to the capsid protein of other animal caliciviruses. Virus Res. 1998, 54, 39–50. [Google Scholar] [CrossRef]
  90. Chen, R.; Neill, J.D.; Prasad, B.V. Crystallization and preliminary crystallographic analysis of San Miguel sea lion virus: An animal calicivirus. J. Struct. Biol. 2003, 141, 143–148. [Google Scholar] [CrossRef]
  91. Chen, R.; Neill, J.D.; Estes, M.K.; Prasad, B.V. X-ray structure of a native calicivirus: Structural insights into antigenic diversity and host specificity. Proc. Natl. Acad. Sci. USA 2006, 103, 8048–8053. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  92. Stuart, A.D.; Brown, T.D. α2,6-linked sialic acid acts as a receptor for feline calicivirus. J. Gen. Virol. 2007, 88 Pt 1, 177–186. [Google Scholar] [CrossRef] [PubMed]
  93. Conley, M.J.; McElwee, M.; Azmi, L.; Gabrielsen, M.; Byron, O.; Goodfellow, I.G.; Bhella, D. Calicivirus VP2 forms a portal-like assembly following receptor engagement. Nature 2019, 565, 377–381. [Google Scholar] [CrossRef]
  94. Lu, Z.; Ledgerwood, E.D.; Hinchman, M.M.; Dick, R.; Parker, J.S.L. Conserved surface residues on the feline calicivirus capsid are essential for interaction with its receptor feline junctional adhesion molecule A (fJAM-A). J Virol. 2018, 92, e00035-18. [Google Scholar] [CrossRef] [PubMed]
  95. Hernández, B.A.; Sandoval-Jaime, C.; Sosnovtsev, S.V.; Green, K.Y.; Gutiérrez-Escolano, A.L. Nucleolin promotes in vitro translation of feline calicivirus genomic RNA. Virology 2016, 489, 51–62. [Google Scholar] [CrossRef]
  96. Alfajaro, M.M.; Cho, E.H.; Park, J.G.; Kim, J.Y.; Soliman, M.; Baek, Y.B.; Kang, M.I.; Park, S.I.; Cho, K.O. Feline calicivirus- and murine norovirus-induced COX-2/PGE2 signaling pathway has proviral effects. PLoS ONE 2018, 13, e0200726. [Google Scholar] [CrossRef]
  97. Yumiketa, Y.; Narita, T.; Inoue, Y.; Sato, G.; Kamitani, W.; Oka, T.; Katayama, K.; Sakaguchi, T.; Tohya, Y. Nonstructural protein p39 of feline calicivirus suppresses host innate immune response by preventing IRF-3 activation. Vet. Microbiol. 2016, 185, 62–67. [Google Scholar] [CrossRef]
  98. Humoud, M.N.; Doyle, N.; Royall, E.; Willcocks, M.M.; Sorgeloos, F.; van Kuppeveld, F.; Roberts, L.O.; Goodfellow, I.G.; Langereis, M.A.; Locker, N. Feline calicivirus infection disrupts assembly of cytoplasmic stress granules and induces G3BP1 cleavage. J. Virol. 2016, 90, 6489–6501. [Google Scholar] [CrossRef]
  99. Wu, H.; Zu, S.; Sun, X.; Liu, Y.; Tian, J.; Qu, L. N-terminal domain of feline calicivirus (FCV) proteinase-polymerase contributes to the inhibition of host cell transcription. Viruses 2016, 8, 199. [Google Scholar] [CrossRef] [PubMed]
  100. Oka, T.; Takagi, H.; Tohya, Y. Development of a novel single step reverse genetics system for feline calicivirus. J. Virol. Methods 2014, 207, 178–181. [Google Scholar] [CrossRef] [PubMed]
  101. Sandoval-Jaime, C.; Green, K.Y.; Sosnovtsev, S.V. Recovery of murine norovirus and feline calicivirus from plasmids encoding EMCV IRES in stable cell lines expressing T7 polymerase. J. Virol. Methods 2015, 217, 1–7. [Google Scholar] [CrossRef] [PubMed]
  102. Afonso, M.M.; Pinchbeck, G.L.; Smith, S.L.; Daly, J.M.; Gaskell, R.M.; Dawson, S.; Radford, A.D. A multi-national European cross-sectional study of feline calicivirus epidemiology, diversity and vaccine cross-reactivity. Vaccine 2017, 35, 2753–2760. [Google Scholar] [CrossRef] [PubMed]
  103. Coyne, K.P.; Gaskell, R.M.; Dawson, S.; Porter, C.J.; Radford, A.D. Evolutionary mechanisms of persistence and diversification of a calicivirus within endemically infected natural host populations. J. Virol. 2007, 81, 1961–1971. [Google Scholar] [CrossRef]
  104. Masubuchi, K.; Wakatsuki, A.; Iwamoto, K.; Takahashi, T.; Kokubu, T.; Shimizu, M. Immunological and genetic characterization of feline caliciviruses used in the development of a new trivalent inactivated vaccine in Japan. J. Vet. Med. Sci. 2010, 72, 1189–1194. [Google Scholar] [CrossRef]
  105. Wensman, J.J.; Samman, A.; Lindhe, A.; Thibault, J.C.; Berndtsson, L.T.; Hosie, M.J. Ability of vaccine strain induced antibodies to neutralize field isolates of caliciviruses from Swedish cats. Acta Vet. Scand. 2015, 57, 86, Erratum in: Acta Vet. Scand. 2016, 58, 14. [Google Scholar] [CrossRef]
  106. Sato, H.; Sehata, G.; Okada, N.; Iwamoto, K.; Masubuchi, K.; Kainuma, R.; Noda, T.; Igarashi, T.; Sawada, T.; Noro, T.; et al. Intranasal immunization with inactivated feline calicivirus particles confers robust protection against homologous virus and suppression against heterologous virus in cats. J. Gen. Virol. 2017, 98, 1730–1738. [Google Scholar] [CrossRef]
  107. Martella, V.; Pinto, P.; Lorusso, E.; Di Martino, B.; Wang, Q.; Larocca, V.; Cavalli, A.; Camero, M.; Decaro, N.; Bányai, K.; et al. Detection and full-length genome characterization of novel canine vesiviruses. Emerg. Infect. Dis. 2015, 21, 1433–1436. [Google Scholar] [CrossRef]
  108. Renshaw, R.W.; Griffing, J.; Weisman, J.; Crofton, L.M.; Laverack, M.A.; Poston, R.P.; Duhamel, G.E.; Dubovi, E.J. Characterization of a vesivirus associated with an outbreak of acute hemorrhagic gastroenteritis in domestic dogs. J. Clin. Microbiol. 2018, 56, e01951-17. [Google Scholar] [CrossRef]
  109. Di Martino, B.; Di Profio, F.; Melegari, I.; Sarchese, V.; Massirio, I.; Luciani, A.; Lanave, G.; Marsilio, F.; Martella, V. Serological and molecular investigation of 2117-like vesiviruses in cats. Arch. Virol. 2018, 163, 197–201. [Google Scholar] [CrossRef]
  110. Plavsic, M.; Shick, K.; Bergmann, K.F.; Mallet, L. Vesivirus 2117: Cell line infectivity range and effectiveness of amplification of a potential adventitious agent in cell culture used for biological production. Biologicals 2016, 44, 540–545. [Google Scholar] [CrossRef]
  111. Conley, M.; Emmott, E.; Orton, R.; Taylor, D.; Carneiro, D.G.; Murata, K.; Goodfellow, I.G.; Hansman, G.S.; Bhella, D. Vesivirus 2117 capsids more closely resemble sapovirus and lagovirus particles than other known vesivirus structures. J. Gen. Virol. 2017, 98, 68–76. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  112. Sosnovtsev, S.V.; Sandoval-Jaime, C.; Parra, G.I.; Tin, C.M.; Jones, R.W.; Soden, J.; Barnes, D.; Freeth, J.; Smith, A.W.; Green, K.Y. Identification of human junctional adhesion molecule 1 as a functional receptor for the Hom-1 calicivirus on human cells. MBio 2017, 8, e00031-17. [Google Scholar] [CrossRef]
  113. Smith, A.W.; Iversen, P.L.; Skilling, D.E.; Stein, D.A.; Bok, K.; Matson, D.O. Vesivirus viremia and seroprevalence in humans. J. Med. Virol. 2006, 78, 693–701. [Google Scholar] [CrossRef] [PubMed]
  114. Lee, H.; Cho, Y.H.; Park, J.S.; Kim, E.C.; Smith, A.W.; Ko, G. Elevated post-transfusion serum transaminase values associated with a highly significant trend for increasing prevalence of anti-Vesivirus antibody in Korean patients. J. Med. Virol. 2012, 84, 1943–1952. [Google Scholar] [CrossRef] [PubMed]
  115. Oliver, S.L.; Asobayire, E.; Dastjerdi, A.M.; Bridger, J.C. Genomic characterization of the unclassified bovine enteric virus Newbury agent-1 (Newbury1) endorses a new genus in the family Caliciviridae. Virology 2006, 350, 240–250. [Google Scholar] [CrossRef] [Green Version]
  116. Cho, E.H.; Soliman, M.; Alfajaro, M.M.; Kim, J.Y.; Seo, J.Y.; Park, J.G.; Kim, D.S.; Baek, Y.B.; Kang, M.I.; Park, S.I.; et al. Bovine nebovirus interacts with a wide spectrum of histo-blood group antigens. J. Virol. 2018, 92, e02160-17. [Google Scholar] [CrossRef]
  117. Di Martino, B.; Di Profio, F.; Martella, V.; Ceci, C.; Marsilio, F. Evidence for recombination in neboviruses. Vet. Microbiol. 2011, 153, 367–372. [Google Scholar] [CrossRef]
  118. Guo, Z.; He, Q.; Yue, H.; Zhang, B.; Tang, C. Genomic characterization of a RdRp-recombinant nebovirus strain with a novel VP1 genotype. Virus Res. 2018, 251, 6–13. [Google Scholar] [CrossRef]
  119. Thomas, C.; Jung, K.; Han, M.G.; Hoet, A.; Scheuer, K.; Wang, Q.; Saif, L.J. Retrospective serosurveillance of bovine norovirus (GIII.2) and nebovirus in cattle from selected feedlots and a veal calf farm in 1999 to 2001 in the United States. Arch. Virol. 2014, 159, 83–90. [Google Scholar] [CrossRef]
  120. Candido, M.; Alencar, A.L.; Almeida-Queiroz, S.R.; Buzinaro, M.G.; Munin, F.S.; Godoy, S.H.; Livonesi, M.C.; Fernandes, A.M.; Sousa, R.L. First detection and molecular characterization of Nebovirus in Brazil. Epidemiol. Infect. 2016, 144, 1876–1878. [Google Scholar] [CrossRef]
  121. Turan, T.; Işıdan, H.; Atasoy, M.O.; Irehan, B. Detection and molecular analysis of bovine enteric norovirus and nebovirus in Turkey. J. Vet. Res. 2018, 62, 129–135. [Google Scholar] [CrossRef] [PubMed]
  122. Pourasgari, F.; Kaplon, J.; Sanchooli, A.; Fremy, C.; Karimi-Naghlani, S.; Otarod, V.; Ambert-Balay, K.; Mojgani, N.; Pothier, P. Molecular prevalence of bovine noroviruses and neboviruses in newborn calves in Iran. Arch. Virol. 2018, 163, 1271–1277. [Google Scholar] [CrossRef]
  123. Park, S.I.; Jeong, C.; Park, S.J.; Kim, H.H.; Jeong, Y.J.; Hyun, B.H.; Chun, Y.H.; Kang, M.I.; Cho, K.O. Molecular detection and characterization of unclassified bovine enteric caliciviruses in South Korea. Vet. Microbiol. 2008, 130, 371–379. [Google Scholar] [CrossRef]
  124. Guo, Z.; He, Q.; Yue, H.; Zhang, B.; Tang, C. First detection of nebovirus and norovirus from cattle in China. Arch. Virol. 2018, 163, 475–478. [Google Scholar] [CrossRef]
  125. Guo, Z.; He, Q.; Zhang, B.; Yue, H.; Tang, C. Detection and molecular characteristics of neboviruses in dairy cows in China. J Gen Virol. 2018. [Google Scholar] [CrossRef]
  126. Farkas, T.; Sestak, K.; Wei, C.; Jiang, X. Characterization of a rhesus monkey calicivirus representing a new genus of Caliciviridae. J. Virol. 2008, 82, 5408–5416. [Google Scholar] [CrossRef]
  127. Farkas, T.; Lun, C.W.; Fey, B. Relationship between genotypes and serotypes of genogroup 1 recoviruses: A model for human norovirus antigenic diversity. J. Gen. Virol. 2014, 95 Pt 7, 1469–1478. [Google Scholar] [CrossRef]
  128. Farkas, T.; Cross, R.W.; Hargitt, E., 3rd; Lerche, N.W.; Morrow, A.L.; Sestak, K. Genetic diversity and histo-blood group antigen interactions of rhesus enteric caliciviruses. J. Virol. 2010, 84, 8617–8625. [Google Scholar] [CrossRef] [PubMed]
  129. Sestak, K. Role of histo-blood group antigens in primate enteric calicivirus infections. World J. Virol. 2014, 3, 18–21. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  130. Zhang, D.; Huang, P.; Zou, L.; Lowary, T.L.; Tan, M.; Jiang, X. Tulane virus recognizes the A type 3 and B histo-blood group antigens. J. Virol. 2015, 89, 1419–1427. [Google Scholar] [CrossRef] [PubMed]
  131. Wei, C.; Farkas, T.; Sestak, K.; Jiang, X. Recovery of infectious virus by transfection of in vitro-generated RNA from tulane calicivirus cDNA. J. Virol. 2008, 82, 11429–11436. [Google Scholar] [CrossRef] [PubMed]
  132. Farkas, T. Rhesus enteric calicivirus surrogate model for human norovirus gastroenteritis. J. Gen. Virol. 2015, 96 Pt 7, 1504–1514. [Google Scholar] [CrossRef]
  133. Chhabra, P.; Ranjan, P.; Cromeans, T.; Sambhara, S.; Vinjé, J. Critical role of RIG-I and MDA5 in early and late stages of Tulane virus infection. J. Gen. Virol. 2017, 98, 1016–1026. [Google Scholar] [CrossRef] [Green Version]
  134. Siqueira, J.D.; Dominguez-Bello, M.G.; Contreras, M.; Lander, O.; Caballero-Arias, H.; Xutao, D.; Noya-Alarcon, O.; Delwart, E. Complex virome in feces from Amerindian children in isolated Amazonian villages. Nat. Commun. 2018, 9, 4270. [Google Scholar] [CrossRef]
  135. Farkas, T.; Wong Ping Lun, C. Prevalence of recovirus-neutralizing antibodies in human serum samples. J. Clin. Microbiol. 2014, 52, 3088–3090. [Google Scholar] [CrossRef]
  136. Kocher, J.F.; Lindesmith, L.C.; Debbink, K.; Beall, A.; Mallory, M.L.; Yount, B.L.; Graham, R.L.; Huynh, J.; Gates, J.E.; Donaldson, E.F.; et al. Bat caliciviruses and human noroviruses are antigenically similar and have overlapping histo-blood group antigen binding profiles. MBio 2018, 9, e00869-18. [Google Scholar] [CrossRef]
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Figure 1. Schematic genome organization of viruses in different genera of the Caliciviridae. (A) The long ORF encodes a polyprotein consisting of seven mostly non-structural proteins (ORF1) and 2–3 structural proteins (ORF2–ORF4). (B) NS3 encodes an NTPase, NS5 the VPg (a structural protein), NS6 a protease, NS7 the RNA-dependent RNA polymerase (RdRp). NS1, NS2 (NS1 + NS2 are also called N-Term), and NS4 have functions in the formation of membranes of the viral replication sites and interact with proteins of the endoplasmic reticulum [32,33]. (C) For Norovirus and Vesivirus ORF2 encodes the major structural protein VP1 (for Vesivirus including a precursor N-terminal leader protein (LC). For Sapovirus, Lagovirus, and Nebovirus the VP1 is derived from the C-terminus of ORF1. ORF2 or ORF3 encode VP2, and ORF4 encodes a protein which has been identified as virulence factor 1 (VF1) for MuNoV. The Nacovirus [28,29], Minovirus [31], and Salovirus [30] genomes have structures as shown in panel C for Lagovirus, Nebovirus, Sapovirus, and Valovirus. From references [24,28,29,30,31], with permission of authors and publisher.
Figure 1. Schematic genome organization of viruses in different genera of the Caliciviridae. (A) The long ORF encodes a polyprotein consisting of seven mostly non-structural proteins (ORF1) and 2–3 structural proteins (ORF2–ORF4). (B) NS3 encodes an NTPase, NS5 the VPg (a structural protein), NS6 a protease, NS7 the RNA-dependent RNA polymerase (RdRp). NS1, NS2 (NS1 + NS2 are also called N-Term), and NS4 have functions in the formation of membranes of the viral replication sites and interact with proteins of the endoplasmic reticulum [32,33]. (C) For Norovirus and Vesivirus ORF2 encodes the major structural protein VP1 (for Vesivirus including a precursor N-terminal leader protein (LC). For Sapovirus, Lagovirus, and Nebovirus the VP1 is derived from the C-terminus of ORF1. ORF2 or ORF3 encode VP2, and ORF4 encodes a protein which has been identified as virulence factor 1 (VF1) for MuNoV. The Nacovirus [28,29], Minovirus [31], and Salovirus [30] genomes have structures as shown in panel C for Lagovirus, Nebovirus, Sapovirus, and Valovirus. From references [24,28,29,30,31], with permission of authors and publisher.
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Figure 2. Pairwise distance distribution histogram of complete VP1 genes of 59 sapoviruses. The peaks of 0–0.159, 0.198–0.471, and 0.522–0.807 correspond to the distance range of strains, genotypes, and genogroups, respectively. The cut-off values for genotype and genogroup clusters were <0.169 and <0.488, respectively, and are indicated by vertical dashed lines. From reference [37], with permission of authors and publisher.
Figure 2. Pairwise distance distribution histogram of complete VP1 genes of 59 sapoviruses. The peaks of 0–0.159, 0.198–0.471, and 0.522–0.807 correspond to the distance range of strains, genotypes, and genogroups, respectively. The cut-off values for genotype and genogroup clusters were <0.169 and <0.488, respectively, and are indicated by vertical dashed lines. From reference [37], with permission of authors and publisher.
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Figure 3. Phylogenetic tree based on nucleotide sequences of complete calicivirus genomes differentiating Valovirus as a separate genus. The tree was constructed by the neighbour-joining method MEGA 3.1. The confidence values at the branch points are based on 1000 bootstrap analyses. The calibration bar indicates distance expressed as nt substitutions per site. Abbreviations: BEC-NB, bovine enteric calicivirus NB/80/US; BEC-Newbury, bovine enteric calicivirus Newbury; EBHSV-GD, European brown hare syndrome virus GD strain; FCV, feline calicivirus; Jena, bovine enteric norovirus strain Jena; Manchester, human sapovirus Manchester; MNV-1, mouse norovirus 1; Norwalk, Norwalk virus; PEC, porcine enteric calicivirus; RHDV-FRG, rabbit haemorrhagic disease virus Germany; SMSV, San Miguel Sea Lion Virus; Tulane, Tulane virus; and St Valérien, St Valérien strains AB90, AB104, F15-10. From reference [25], with permission of authors and publisher.
Figure 3. Phylogenetic tree based on nucleotide sequences of complete calicivirus genomes differentiating Valovirus as a separate genus. The tree was constructed by the neighbour-joining method MEGA 3.1. The confidence values at the branch points are based on 1000 bootstrap analyses. The calibration bar indicates distance expressed as nt substitutions per site. Abbreviations: BEC-NB, bovine enteric calicivirus NB/80/US; BEC-Newbury, bovine enteric calicivirus Newbury; EBHSV-GD, European brown hare syndrome virus GD strain; FCV, feline calicivirus; Jena, bovine enteric norovirus strain Jena; Manchester, human sapovirus Manchester; MNV-1, mouse norovirus 1; Norwalk, Norwalk virus; PEC, porcine enteric calicivirus; RHDV-FRG, rabbit haemorrhagic disease virus Germany; SMSV, San Miguel Sea Lion Virus; Tulane, Tulane virus; and St Valérien, St Valérien strains AB90, AB104, F15-10. From reference [25], with permission of authors and publisher.
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Figure 4. Phylogenetic relationship between the Nacovirus genus and other genera of the Caliciviridae, based on full length amino acid sequences of VP1, the major capsid protein. The calibration bar indicates genetic distance. Abbreviations: CaCv, canine calicivirus; ChCV, chicken calicivirus Bavaria; Ch-F10026n, chicken calicivirus F10026n; CV-2117, calicivirus 2117; EBHSV, European brown hare syndrome virus; FCV, feline calicivirus; GoCV, goose calicivirus; MCV, mink calicivirus; Newbury1, Newbury-1 virus; NoV, norovirus; RHDV, rabbit haemorrhagic disease virus; SaV, sapovirus; St Valérien, St Valérien virus; TuCV, turkey calicivirus; TulaV, Tulane virus; VESV, vesicular exanthema of swine virus. From reference [29], with permission of authors and publisher.
Figure 4. Phylogenetic relationship between the Nacovirus genus and other genera of the Caliciviridae, based on full length amino acid sequences of VP1, the major capsid protein. The calibration bar indicates genetic distance. Abbreviations: CaCv, canine calicivirus; ChCV, chicken calicivirus Bavaria; Ch-F10026n, chicken calicivirus F10026n; CV-2117, calicivirus 2117; EBHSV, European brown hare syndrome virus; FCV, feline calicivirus; GoCV, goose calicivirus; MCV, mink calicivirus; Newbury1, Newbury-1 virus; NoV, norovirus; RHDV, rabbit haemorrhagic disease virus; SaV, sapovirus; St Valérien, St Valérien virus; TuCV, turkey calicivirus; TulaV, Tulane virus; VESV, vesicular exanthema of swine virus. From reference [29], with permission of authors and publisher.
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Table
Table 1. Calicivirus classification including genera and type species (and abbreviations used).
Table 1. Calicivirus classification including genera and type species (and abbreviations used).
GenusType Species
Established:
Norovirus (NoV)Norwalk virus (NV)
Sapovirus (SaV)Sapporo virus (SV)
Lagovirus (LaV)Rabbit hemorrhagic disease virus (RHDV)
European brown hare syndrome virus (EBHSV)
Vesivirus (VeV)Vesicular exanthema of swine virus (VESV)
Feline calicivirus (FCV)
San Miguel sea lion virus (SMSV)
Nebovirus (NeV)Newbury-1 virus (NBV)
Proposed:
Recovirus (ReV)Tulane virus (simian)
Valovirus (VaV)St Valérian virus (porcine)
Bavovirus (BaV)Bayern virus (avian)
Nacovirus (NaV)Novel avian calicivirus (chicken, turkey)
Salovirus (SaV)Atlantic salmon calicivirus (salmon)
Minovirus (MiV)Fathead minnow calicivirus (minnow)
Modified from: http://ictvonline.org/virusTaxonomy.asp 2018 and references [24,25,26,27,28,29,30,31].
Table
Table 2. Tools available for comprehensive study of different genera of the Caliciviridae.
Table 2. Tools available for comprehensive study of different genera of the Caliciviridae.
GenusCell/Enteroid CultureHelper Virus-Free RG SystemAnimal Model
Norovirus
MuNoV+ [1]+ [2,3,4,5]+ [6,7,8,9]
HuNoV+ [10,11](+) to be published(+) [12]
Sapovirus+ porcine [46]+ [55]+ [37]
- human [47]
Lagovirus+ [69]+ [70]+ [75]
Vesivirus+ [86,87,110]+ [100,101]+ [103]
Nebovirus  To be done  To be done  To be done
Recovirus+ [128]+ [131]  To be done
The genera Valovirus, Bavovirus, Nacovirus, Minovirus, and Salovirus have only recently been identified, and the techniques mentioned above have to be developed.

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Desselberger, U. Caliciviridae Other Than Noroviruses. Viruses 2019, 11, 286. https://doi.org/10.3390/v11030286

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Desselberger U. Caliciviridae Other Than Noroviruses. Viruses. 2019; 11(3):286. https://doi.org/10.3390/v11030286

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Desselberger, Ulrich. 2019. "Caliciviridae Other Than Noroviruses" Viruses 11, no. 3: 286. https://doi.org/10.3390/v11030286

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