Figures
Abstract
Background
Tissue culture-adapted Tulane virus (TV), a GI.1 rhesus enteric calicivirus (ReCV), and a mixture of GII.2 and GII.4 human norovirus (NoV)-containing stool sample were used to intrastomacheally inoculate juvenile rhesus macaques (Macaca mulatta) in order to evaluate infection caused by these viruses.
Methodology & Findings
Two of the three TV-inoculated macaques developed diarrhea, fever, virus-shedding in stools, inflammation of duodenum and 16-fold increase of TV-neutralizing (VN) serum antibodies but no vomiting or viremia. No VN-antibody responses could be detected against a GI.2 ReCV strain FT285, suggesting that TV and FT285 represent different ReCV serotypes. Both NoV-inoculated macaques remained asymptomatic but with demonstrable virus shedding in one animal. Examination of duodenum biopsies of the TV-inoculated macaques showed lymphocytic infiltration of the lamina propria and villous blunting. TV antigen-positive (TV+) cells were detected in the lamina propria. In most of the TV+ cells TV co-localized perinuclearly with calnexin – an endoplasmic reticulum protein. A few CD20+TV+ double-positive B cells were also identified in duodenum. To corroborate the authenticity of CD20+TV+ B cells, in vitro cultures of peripheral blood mononuclear cells (PBMCs) from healthy macaques were inoculated with TV. Multicolor flow cytometry confirmed the presence of TV antigen-containing B cells of predominantly CD20+HLA-DR+ phenotype. A 2-log increase of viral RNA by 6 days post inoculation (p<0.05) suggested active TV replication in cultured lymphocytes.
Citation: Sestak K, Feely S, Fey B, Dufour J, Hargitt E, Alvarez X, et al. (2012) Experimental Inoculation of Juvenile Rhesus Macaques with Primate Enteric Caliciviruses. PLoS ONE 7(5): e37973. https://doi.org/10.1371/journal.pone.0037973
Editor: D. William Cameron, University of Ottawa, Canada
Received: February 3, 2012; Accepted: April 27, 2012; Published: May 30, 2012
Copyright: © 2012 Sestak et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This work was supported by grants from the National Institutes of Health R21RR024871, P51RR000164 and U24RR018111 to KS, and P01HD013021 and the Infectious Disease Scholar Fund of CCHMC to TF. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Introduction
Caliciviruses (CV) are small, non-enveloped, icosahedral viruses with a ∼7.5–8.5 kb positive sense, single stranded, polyadenylated RNA genome. The Caliciviridae family consists of five established genera, Norovirus, Sapovirus, Lagovirus, Vesivirus and Nebovirus. Rhesus enteric CVs (Recovirus), St. Valerian-like viruses (Valovirus) and chicken CVs represent three additional, yet unassigned CV genera [1]–[3]. Noroviruses (NoV) are important etiologic agents of acute gastroenteritis in humans and account for the majority of nonbacterial gastroenteritis outbreaks as well as >50% of all food-related gastroenteritis outbreaks [4], [5]. NoVs can be subdivided into five genogroups (GI-V) and at least 33 genotypes [6], [7]. No robust cell culture or in vivo model exists to study human NoVs.
The first attempt to develop a primate model for human NoV gastroenteritis dates back to 1978 when Wyatt and colleagues induced asymptomatic infection of chimpanzees by the Norwalk virus [8]. Since then, further efforts have been made with porcine, bovine, murine and other animal hosts including non-human primate (NHP) species to establish a model that would resemble human NoV gastroenteritis [9]–[26]. Despite that substantial achievements have been made with these models, there is still a demand for another alternative that would simultaneously address human NoV-induced clinical illness as well as reflect biological features of human NoVs including their genetic, antigenic and HBGA diversity while being utilized in vivo and in vitro.
Our group recently discovered and characterized a new group of enteric CVs of rhesus monkey host origin with the proposed name Recoviruses (ReCVs) [1], [27], [28]. Enteric CVs frequently infect colonies with captive NHPs [1], [19], [27], [29], [30]. These reports are based on detection of serum antibodies, electron microscopy or presence of viral RNA in stool samples. The extent of ReCV seroprevalence measured by VN antibodies (as high as 80%) in NHPs colonies is conditioned by host species, age, type of housing and colony [Sestak and Farkas, unpublished]. It is not clear, however, if reactivity of NHP serum samples with human NoVs reflects CV interspecies transmission or cross-reactivity between CVs of different primate hosts [19], [27]. Studies conducted with human NoV-inoculated NHPs suggest that there are differences in susceptibility to infection not only among different host species but also within species – likely caused by individual genetic resistance factors although possible differences in adaptive immunity play an important role as well. While some primates remain asymptomatic after infection, others exhibit diarrhea, vomiting, and dehydration, resembling the clinical course of human NoV gastroenteritis [8], [10], [12], [31]. Robust, virus-specific seroconversion and virus shedding in stools up to three weeks post inoculation have only been reproduced in NHPs. In order to induce symptomatic infection, serological and HBGA pre-screening of candidate animals need to be considered prior to experimental challenge. The main objective of this study was to explore the suitability of juvenile rhesus macaques as a TV infection model to study enteric calicivirus replication, pathogenesis and immunity.
Results
Experimental inoculation of juvenile rhesus macaques with TV induces clinical symptoms of disease
Intragastric inoculation of TV of two of the three juvenile macaques (HC55 and HI77) resulted in diarrhea and fever within two days after virus inoculation (Fig. 1) whereas no clinical symptoms were observed for HB61 despite that all three macaques shed TV. The presence of viral genome was measured in cell-free plasma by qRT-PCR. No vomiting and viremia was detected in any of the animals. All three TV-inoculated animals shed the virus for at least 8 days with peak shedding levels of >105 TV-RNA copies per gram of stools in HB61 and HC55 and ≥104 TV-RNA copies per gram of stools in HI77 (Fig. 2). Considering that juvenile macaques produce on average 80±20 grams of stool daily, the amount of virus shed in HC55 and HB61 macaques exceeded the amount received via inoculum (Tables 1 and 2).
Stool consistency measurements indicate onset of diarrhea (>1.0 red line cut-off) upon inoculation. Two of the three TV-inoculated macaques (HC55 and HI77) showed symptoms of diarrhea up to post-inoculation day (PID) 6 and 8. The two human NoV-inoculated animals (GI96 and HB11) did not show diarrhea. HC55 and HI77 macaques developed elevated body temperature (>102.5 F; red line cut-off) during the first two weeks following TV inoculation, while body temperatures of the other animals remained normal. Definition of diarrhea scale: (0 = normal/dry, 0.5 = normal, 1.0 = normal/soft, 1.5 = pasty, 2.0 = semiliquid, 2.5 = watery), and fever: (<102.5 = normal, 102.5 = borderline, >102.5 = fever).
All of the three TV-inoculated macaques showed presence of virus-specific RNA in stools (upper panel) and developed VN antibody responses (≥4-fold increase) by PID 7 (lower panel). Duration of shedding ranged in TV-inoculated macaques between 8–10 days while reaching the peak of ∼105 RNA copies per gram of stools in HB61 and HC55 and ∼104 in HI77. The detection limit of the assay was 10–100 copies per reaction. Antibody serum levels reached their peak in all three macaques by PID 7–9 (1∶160–1∶640) while returned to pre-inoculation levels by PID 80.
No clinical symptoms of diarrhea and fever were observed in the two NoV-inoculated macaques although GI96 met at one time point the definition of “borderline” fever (102.5 F). Viral RNA was detected in fecal specimens from macaque HB11 up to PID 13 and macaque GI96 up to PID 4 by strain-specific nested RT-PCR (Table 2). Both GII.2 and GII.4 viruses were shed in macaque HB11 while only GII.2 virus was detected in macaque GI96. Likely because a lower sensitivity of the quantitative real-time RT-PCR (20–200 RNA copies for GII strains per reaction) compared to nested RT-PCR, only PID 1, 2 and 9 samples from HB11 but none of the samples from GI96 could be evaluated quantitatively (Table 2). Considering that juvenile rhesus macaques of 2.5–4.0 years of age produce daily 80±20 grams of stool, the HB11 macaque produced more virus in stools than what was received in inoculum.
Serum antibody responses to TV
All three TV-inoculated macaques developed a VN serum antibody response (≥4-fold increase) by PID 7 (Fig. 2). VN antibodies reached their peak at PID 7–9 (1∶160–1∶640), persisted at their peak levels up to PID 30–38 after which they gradually started to decline (Fig. 2). By PID 80, VN antibody levels in all three TV-inoculated animals dropped to almost pre-inoculation levels. None of the TV (GI.1 genotype)-inoculated animals developed VN antibody response against FT285–a GI.2 ReCV. A rise in NoV-specific antibody responses against Minerva (GII.4) VLPs could not be detected in the NoV-inoculated macaques (HB11 and GI96) which had consistent anti-Minerva serum ELISA antibody titers of 1∶50 and 1∶800 throughout the experiment, respectively.
Histopathological changes in small intestine
H&E-stained duodenum tissues from TV- and NoV-inoculated macaques were compared with tissues from normal, healthy, age-matched controls (Fig. 3). While no significant damage was seen in the intestinal epithelium, in both TV- and NoV-inoculated animals, mononuclear, lymphocytic infiltration was observed in the lamina propria. In addition, moderate blunting and distention of the villi was observed in all three TV-inoculated animals (Fig. 3). No histopathological lesions were observed in control macaque intestinal tissues.
A– Duodenum tissue from healthy control macaque with normal tissue architecture of intestinal villi. Magnification 10x. B– Duodenum tissue obtained at PID 3 from TV-inoculated HC55 macaque: Superficial mucosa contains diffuse mononuclear cell infiltrate with formation of an intra-epithelial lymphoid follicle. Villi are slightly blunted. Magnification 10x. C– Superficial mucosa of TV-inoculated macaque contains macrophages, plasma cells and scattered eosinophils. Magnification 40x. D– The brush border (green lining = villi) was preserved in TV-inoculated macaques. Purple blue cells indicate underlying subepithelium (TG2 is a digestive enzyme).
Visualization of TV in small intestinal biopsies
In order to visualize and to characterize TV-infected cells directly in small intestine, duodenum biopsies were collected at PID 3 and studied by confocal microscopy. Antibodies specific to human T-, B-, epithelial, dendritic, apoptotic cells as well as macrophages and endoplasmic protein calnexin were used in conjunction with TV antibodies (Figs. 4 and 5). Consistent with the histopathological findings, no TV antigen was detected in epithelial cells. Nevertheless, numerous TV+ cells were observed within the lamina propria. No TV+ cells were detected in biopsies from uninfected control macaques (Fig. S1). Many of the TV antigens exhibited perinuclear fluorescence while TV-specific antibodies colocalized with calnexin in some cells (Fig. 5; Fig. S2). Some of the TV+ cells also stained with CD20, a B cell-specific marker (Fig. 4C).
A– The cytokeratin+ epithelial cells (red) did not co-localize with TV (green). The TV+ cells appear in subepithelium i.e. lamina propria (arrows). B– The subepithelial CD3+ T lymphocytes (red) did not co-localize with TV (green). C– Co-localization of some of the CD20+ B cells (red) with TV (green) is indicated by arrows. D– The IBA-1+ macrophages (red) did not co-localize with TV (green). Nuclear DNA is in blue. E– The CD11c+ myeloid dendritic cells (red) did not co-localize with TV (green) while co-localization between CD11c+ and calnexin (blue) markers resulted in purple cell coloration. The co-localization of TV+ cells with calnexin is indicated by arrows. F– Absence of co-localization between TV (green) and TUNEL (red) markers indicates that TV-infected cells did not undergo apoptosis. Differential interference contrast (gray) is highlighted for the better visualization of tissue architecture.
A– While most of the cells are calnexin-single-positive, simultaneous presence of both TV (green) and calnexin (red) antigens is seen in some of the (yellowish) cells. DIC– differential interference contrast. B– Spectral overlap of TV and calnexin antigens is shown by arrows.
Quantitative analysis of in vitro TV-inoculated PBMCs
Because suitability of intestinal endoscopic (pin-head size) biopsies for quantitative cell phenotypic analysis by confocal microscopy is limited, in vitro experiments with TV-inoculated PBMCs obtained from eight healthy macaques were performed to corroborate the presence of CD20+TV+ B cells in the biopsy samples and to assess the susceptibility of mononuclear cell populations such as T and B lymphocytes to TV infection. In vitro cultures of PBMCs from 8 healthy rhesus macaques were used. TV and negative control media-inoculated cells were harvested at 2 h, 24 h and 6 days PI and tested by multicolor flow cytometry and/or qPCR to determine the number of TV+ cells and virus load. Two populations of interest were identified by flow cytometry: CD3+ T and CD20+ B cells (Fig. 6A). Based on distinct subset of CD20+TV+ cells identified within CD20+ B cell population (Fig. 6A), presented data focus on B cells while T cell populations and negative controls are shown for comparison (Fig. 6B, Fig. 7). The two “parent” (CD20+ and CD3+) populations were further sub-divided into CD20+HLA-DR+, CD20+CD11c+, CD20+CD123+, CD3+HLA-DR+ and CD3+CD11c+ cells, corresponding to five different B and T cell subsets, to determine which of these cells, if any, contained the TV. The distribution of five of the above lymphocyte subsets was similar between TV-inoculated and media control PBMCs, as well as between cultures harvested at 24 h and 6 days PI, with CD20+HLA-DR+ B cell subset being the dominant (Fig. 7A, C). In both CD3+ and CD20+ cell populations HLA-DR+ cells were the most abundant, representing over 90% of cells while CD11c+ and/or CD123+ cells represented less than 10%. All of the five lymphocyte subsets contained TV+ cells, but only the CD20+HLA-DR+TV+ cells surpassed 2% (p>0.05) of the parent (CD20+HLA-DR+) population at 24 h PI (Fig. 7B). Moreover, the proportion of CD20+HLA-DR+TV+ cells increased to >6% (p<0.05) of the parent population by PID 6 (Fig. 7D). Such an increased proportion of TV+ cells in cultured PBMCs was corroborated by qPCR. A significant increase in virus load was detected within 1–6 days PI while no virus was detected in non-inoculated controls: The average viral RNA copy number per well by PID 1 (1.3×106) and PID 6 (2.8×106) was higher (p<0.05) than the RNA copy number measured by 2 hours PI (2.3×105).
A– PBMCs isolated from healthy rhesus macaques were used for in vitro inoculation with TV. After being cultured in vitro for 6 days, cells were sorted out into CD3+ T cell and CD20+ B cell populations. Presence of TV antigens was detected in CD20+ B cells as shown by histograms (black peak). B– The CD20+ B cells were further subdivided into populations expressing the HLA-DR, CD11c or CD123 antigens. Presence of TV was revealed predominantly in CD20+HLA-DR+ cells while some of the other lymphocyte populations including the CD20+CD11c+ and CD20+CD123+ B cells also contained TV antigens.
A & B– One day-old cultures of TV-inoculated PBMCs show the trend (p>0.05) for TV antigen expression by CD20+HLA-DR+ B cells. C & D– Six days-old cultures show significant presence of TV antigens predominantly inside the CD20+HLA-DR+ cells (p<0.05). Several other T and B cell subsets also contain TV while no virus was detected in negative control, mock-inoculated PBMCs. Asterisks indicate significant differences between the TV-inoculated and control cells.
Discussion
Human NoVs are a common cause of epidemic and sporadic acute gastroenteritis worldwide [4], [32]. The prototype Norwalk virus was discovered in 1972 [33], however NoV research and the development of prevention strategies have since been hampered by the lack of robust cell culture system and animal model that closely mimics the clinical symptoms of NoV gastroenteritis in humans. Despite these difficulties, NoV VLP vaccines are in early phase clinical trials [34], [35]. Evaluation of these vaccines largely depends on challenge studies in human volunteers.
Development of an animal model for human NoV gastroenteritis might be based on infection of animals with human NoVs or the use of cultivable animal CVs as surrogates. Attempts to experimentally induce human NoV infection in NHP species such as common marmosets, cotton top tamarins, cynomolgus macaques, pigtail macaques, rhesus macaques and chimpanzees almost invariably resulted in asymptomatic infections [8], [10], [12], [31]. In one study however, a symptomatic infection characterized by diarrhea and vomiting of newborn pigtail macaques was induced following inoculation with the Toronto virus [12], but these results have not been confirmed by other studies. Moreover, detection of CVs or CV antibodies, including NoVs was reported in colonies with captive NHPs [27], [29], [30], [36]. In captive NHP colonies, CVs have been detected in stool samples of animals with symptoms of diarrhea. Recent data suggest an ∼80% ReCV seroprevalence in rhesus macaques housed at three separate U.S. colonies [27, Sestak and Farkas, unpublished]. While ReCV seroprevalence rates are high in juvenile and adult rhesus monkeys, other NHP species exhibit different and/or lower seroprevalence rates. As suggested, these differences could be due to species-specific susceptibility/resistance factors such as HBGAs [19]. Considering the high TV seroprevalence combined with high rates of juvenile diarrhea-associated morbidity in these colonies, it is suspected that ReCV infections play an important role in the etiology of NHP gastroenteritis. Here we examined for the first time whether experimental challenge of juvenile rhesus macaques with the tissue culture-adapted prototype ReCV (TV) induces clinical disease. Although no equivalent inoculum of tissue culture-adapted human NoV was available, two additional animals were challenged with human NoV stool suspensions to compare the clinical outcome between TV- and human NoV-inoculated animals. In order to increase the chance of infection, both animals were inoculated with a mixture of GII.2 and GII.4 NoVs. Mixed NoV infections have been described in oyster-associated human NoV outbreaks [37]. Also, the existence of recombinant NoVs [38] indicates that mixed NoV infections do frequently take place.
Two out of three TV-inoculated macaques developed symptoms of gastroenteritis (diarrhea, fever and virus shedding in stools but no vomiting or reduced appetite were noticed) while the third remained asymptomatic. All three animals shed virus for more than a week (8–10 PID) even though maximum virus shedding reached ∼105 viral copies per gram of stool only in HC55 and HB61. Quantitative evaluation of virus shed in these two macaques combined with the daily output of stools (Table 2) indicate that the amount of virus shed exceeded the amount of virus in the inoculum. Vomiting was not detected as a clinical sign of TV infection. This could be due to small number of animals in this study or other reasons. Studies with NoV-infected children suggest that ∼25–30% of these children do not vomit [39], [40]. In addition, still unknown differences between ReCV and NoV pathogenesis might also be linked with the lack of vomiting in TV-infected macaques.
All three TV-inoculated macaques developed ≥4 fold TV-specific VN antibody responses within 7 days PI, indicating an early memory response, consistent with low levels of VN antibodies prior to inoculation. VN antibodies reached their peak by PID 7–9 in all of the three animals and persisted at high levels up to 4–5 weeks PI. After 5 weeks PI, VN antibody titers started to decline, possibly due to absence of re-exposure(s) that take place in colony animals [14], [18]. It is also possible that the binding (ELISA) antibodies would be detected for much longer period of time than functional (VN) antibodies. Finally, it is important to highlight that the low levels (1∶40–1∶80) of VN antibodies were still present at the end of the study in TV-inoculated macaques. Consistent with these results, declining NoV immunity has also been observed in human volunteers [41], [42]. Thus, questions still remain regarding the longevity, magnitude, class and role of CV antibodies in protection.
Interestingly, VN antibody responses could not be detected in any of the TV-infected animals against FT285 a GI.2 ReCV isolate, indicating that the two strains likely belong to different serotypes. TV and FT285 ORF2 and capsid proteins share 69% nt and 74% aa homology (Farkas and Sestak unpublished), which is comparable with differences between different human NoV genotypes. If humoral immunity plays a role in protection against enteric CV infections, our results are translational for NoV vaccine design since multiple genetic types have been described for both ReCVs and human NoVs. At present, ∼10 cell culture-adapted ReCVs representing at least three genotypes are available in our laboratory. Consistent with previous reports, none of the two human NoVs used in this study caused clinical infection. Since all macaques secreted type-B HBGA in their saliva (not shown), and both NoV challenge strains were obtained from a type-B patient, it was predicted that both strains would replicate in macaques. However, only GII.2 virus was detected in macaque GI96, while both Gll.2 and Gll.4 viruses were shed by HB11 (Table 2). Although duration of shedding in HB11 was suggestive of virus replication, no antibody responses were detected against Minerva (GII.4) VLPs. Macaque GI96 had relatively high level (1∶800) of ELISA antibodies at the beginning of the study. This could explain the complete absence of GII.4 virus shedding in GI96. GII.2 VLPs were not available to evaluate the GII.2-specific seroresponses in this study. Low viral loads in stools of Norwalk virus-challenged rhesus macaques were also reported by Rockx and colleagues [10]. In their study, two animals stopped shedding virus by PID 2 while one animal shed up to PID 19 while it developed strong antibody responses. In the same study, marmosets and tamarins, but not cynomolgus macaques, shed the virus up to PID 4 but did not develop antibody responses. Taken together, these studies indicate that NHPs can be subclinically infected with human NoVs but the infection is very limited and its intensity varies in different species and individuals.
Histopathological examination of H&E-stained duodenum biopsies obtained at PID 3 demonstrated lymphocytic infiltration of the lamina propria in all five inoculated macaques while mild villous blunting was present in three TV-inoculated macaques. These signs were consistent to some degree with reported histopathology of NoV-infected humans [43]–[45]. Although no ultrastructural examination of enterocytes was performed by transmission electron microscopy, confocal microscopy examination of intestinal brush border and epithelial layer revealed no significant damage of enterocytes indicating the possibility that virus might have translocated into lamina propria without replicating in enterocytes. This finding differs from what was reported with human NoV-inoculated gnotobiotic pigs or calves that showed presence of viral particles inside the enterocytes by PID 3 [9], [46]. Notwithstanding, our results are consistent with reported findings of human NoV i.v.-inoculated chimpanzees which showed the presence of NoV antigens in intestinal lamina propria while exhibiting the signs of asymptomatic virus infection such as virus shedding in stools and seroconversion [31]. In all of these studies, enterocyte damage was minimal or undetectable regardless of the detection of virus antigen raising questions about CV pathogenesis and their exact host cell tropism. In case of TV-inoculated macaques, TV antigen-containing cells with perinuclear fluorescence were found in intestinal lamina propria (Figs. 4 and 5). In many of these cells TV-specific antibodies co-localized with calnexin, an endoplasmic reticulum marker, consistent with the formation of replication complexes reported for feline CV [47].
To determine the authenticity of TV-containing cells, several of the human-specific cell markers were utilized (Table 3). A few CD20+TV+ B lymphocytes were identified directly in duodenum lamina propria by confocal microscopy. Since suitability of intestinal pin-head-sized biopsies for quantitative cell phenotype analysis by confocal microscopy is limited, in vitro experiment with TV-inoculated PBMCs obtained from eight healthy macaques was performed, utilizing quantitative multicolor flow cytometry, to determine if CD20+TV+ B cells could be identified in these cultures (Figs. 6 and 7). The presence of CD20+TV+ B cells was demonstrated corroborating the confocal microscopy data. Most of the TV+ cells expressed HLA-DR antigen, suggesting a) involvement of TV+ lymphocytes in antigen presentation to other immune cells or b) possibility of activated lymphocytes being infected. Increased viral RNA load (p<0.05) that was detected in cultured PBMCs within 24 h following TV inoculation supported the flow cytometry data and was suggestive of virus replication. In study by Lay and colleagues, Norwalk virus failed to replicate in macrophages or dendritic cells derived from human peripheral blood [48]. A more recent study by Chan and colleagues indicates however that human NoV binds to the lamina propria and Brunner's gland cells of the human duodenum [49]. We have also incorporated CD123 marker to determine whether some B cells start to acquire dendritic cell (DC)-like features following their in vitro exposure to virus. Earlier reports by Bjorck and colleagues (1998) showed that CD19+ B cells can differentiate into DCs following cytokine stimulation [50]. Although commonly used as a DC marker, CD11c is also expressed by activated or leukemic B cells [51], [52]. Recently, a subpopulation of memory B cells was shown to express CD11c [53]. In our study we observed increased CD11c expression by TV-infected B cells suggesting the activation of these cells following TV infection.
The fact that TV was identified in both B and T cells is to some degree different from findings reported for murine NoVs that replicate efficiently in macrophage and dendritic cell lines [13], [25], [26]. Since Rhesus CD14+ cells can differentiate into dendritic cells in vitro, it will be interesting to evaluate if these cells will become permissive to TV infection. In summary, our results are consistent with findings of human NoV -infected chimpanzees that remained asymptomatic but showed the presence of NoV antigen in intestinal lamina propria [31]. Many features of CV infection in primates such as HBGA-associated genetic susceptibility to infection remain to be elucidated. In this proof-of-concept study, we demonstrated the potential of rhesus macaques using ReCV as a diarrheal disease model for human NoV. In future studies candidate animals will be selected by prescreening for the specific HBGAs and/or by using newborn SPF or animals completely naïve of previous ReCV exposure while using highly cytopathic ReCV strain for challenge.
Materials and Methods
Ethics statement
Approval for all veterinary procedures in this study had been obtained from the Tulane University Animal Care and Use Committee, Animal Welfare Assurance A-4499-01. Animals in this project were under the full care of veterinarians with the standards incorporated in the Guide to the Care and Use of Laboratory Animals (NIH) 78-23 (Revised, 1996). All veterinary procedures were performed only with sedated animals. Animal welfare and steps were taken to ameliorate suffering in accordance with the recommendations of the Weatherall report. The findings and conclusions in this article are those of the authors and do not necessarily represent the views of the Centers for Disease Control and Prevention. This article did receive clearance through the appropriate channels at the CDC prior to submission.
Animals, procedures and samples collected
Forty juvenile (<4 years-old) candidate rhesus macaques were identified from a group of 300 based on absence of TV-neutralizing serum antibodies [27]. Due to unrelated reasons, selected candidate animals were assigned for the study not immediately but after a delay, which resulted in low, marginal but detectable TV seroconversion. Five animals (1∶10–1∶40 VN antibodies) with no detectable virus shedding in feces were included in this study (Table 1). Only simian retrovirus- (SIV, SR and STLV) and enteric pathogen-free animals were selected using the diagnostic techniques described elsewhere [54], [55]. All five macaques were inoculated intragastrically and were housed under biosafety level two (BSL2) conditions. Three macaques were inoculated with tissue culture-adapted TV and two macaques with bacteria-free stool suspensions containing a mixture of GII.2 an GII.4 NoVs (Table 1). Human NoV positive stool samples (NF2002 and NF2003; GenBank accession numbers: JQ320072 and JQ320073) were collected during two family outbreaks occurring in May 2002 and March 2003 in Cincinnati, OH, respectively. The inoculum was prepared from 20% (w/v) stool suspensions that were clarified by low-speed centrifugation and filtered using 0.22 μm filters. Aliquots were stored at −80°C. Upon inoculation, body temperature and stool consistency were recorded daily up to post-inoculation day (PID) 40. Stool samples were collected each morning at indicated time points (Fig. 1) from the individual cage pans that were replaced daily. Diarrhea was defined above the score of 1.0 according to following key: (0 = normal/dry, 0.5 = normal, 1.0 = normal/soft, 1.5 = pasty, 2.0 = semiliquid, 2.5 = watery), while fever was defined above the 102.5 F: (<102.5 = normal, 102.5 = borderline, >102.5 = fever).
Samples of blood and plasma were obtained weekly and/or at indicated time points (Fig. 2) up to PID 80. Based on similar experiments with gnotobiotic piglets [14], pediatric endoscopy method was used at PID 3 to obtain ten pin-head-sized biopsies from the distal duodenum of all five inoculated and two negative control healthy macaques [56].
Virus antibody assays
Plasma samples collected from all five macaques were tested for the presence of virus-specific antibodies. TV-inoculated macaques (HC55, HI77 and HB61) were tested for the presence and magnitude of TV virus-neutralizing (VN) antibodies [27]. Briefly, serum samples were titrated in duplicate wells of 96-well tissue culture plates (Corning Life Sciences, Lowell, MA) to neutralize 100 TCID50 TV (GI.1) or FT285 (GI.2) ReCVs. To avoid non-specific neutralization by complement, serum samples were heat inactivated. Virus/serum mix was incubated at 37°C for 1 h and transferred into wells seeded with 1×104 LLC-MK2 cells/well in duplicate one day prior. Plates were stained with crystal violet at 72 h post infection (Sigma-Aldrich, St. Louis, MO). At this time point, all cells in the virus control exhibited CPE characterized by cellular degeneration and detachment. VN antibody titer was determined as the highest dilution of the serum sample at which the cell monolayer was at least 50% intact in duplicate wells.
Human NoV-inoculated macaques (HB11 and GI96) were tested for the presence of NoV-binding (ELISA) antibodies using human NoV GII.4 (Minerva) virus-like particles (VLPs), as described previously [27]. Briefly, VLPs diluted in PBS were coated onto 96-well microtiter plates (Dynex, Immulon, Dynatech) at 50 ng/well, overnight, at 4°C. Every second row of the 96-well plate was left uncoated and served as background control. Plates were blocked with 10% Blotto-PBS for 1 h at 37°C. Serum samples, two-fold diluted in 1% Blotto-PBS, starting from 1∶50 were added to two wells each, and the plates were incubated for 1 h at 37°C. Horseradish peroxidase (HRP)-conjugated goat anti-rhesus IgG (H+L) (Southern Biotech, Birmingham, AL) was added at 1∶3,500 dilution in 1% Blotto-PBS, and the plates were incubated for 1 h at 37°C. Following each step, the plates were washed five times with PBS-0.05% Tween 20 in an automated plate washer (ELx 405 Auto Plate Washer, Bio-tek Instruments Inc., Winooski, VT). Finally, TMB substrate (BD Biosciences, San Jose, CA) was added, the plates were incubated for 10 min at room temperature and the color development was stopped by 1 M H3PO4. Optical density (OD) values were recorded by the use of Tecan Spectra II microtiter plate reader (Tecan AG, Switzerland) at 450 nm. OD readings for each serum sample/dilution were determined as the average of difference between values obtained in the two VLP-coated and two uncoated wells. The cut-off was determined as the mean plus two standard deviations of the OD readings of the control (uncoated) wells.
Histopathology, immunohistochemistry and confocal microscopy
Duodenum biopsies collected at PID 3 were used for histopathological evaluation of tissue architecture following the standard H&E staining method [56]. In addition, antibodies specific to primate T and B lymphocytes, epithelial cells, macrophages, myeloid dendritic cells, apoptotic cells and endoplasmic reticulum protein calnexin (Table 3) were used in conjunction with TV-specific antibodies (rhesus serum of ≥1∶1,280 VN antibody titer), to identify the potential TV-infected cells according to described immunohistochemistry protocols [56], [57].
TV infection of peripheral blood mononuclear cells (PBMC) with TV
PBMCs were isolated from whole blood of 8 healthy, normal rhesus macaques by density gradient centrifugation using Lymphocyte Separation Medium (MP Biomedicals, LLC, Santa Ana, CA) and seeded in 24-well cell culture plates coated with collagen (BD Biosciences, San Diego, CA) at a concentration of 2×106 cells per well. Cells were cultured at 37°C, 5% CO2 in RPMI 1640 medium containing 2 mM glutamine, 1 mM sodium pyruvate, 100 U/ml penicillin, and 100 mg/ml streptomycin (Mediatech, Inc., Manassas, VA) supplemented with 10% heat-inactivated FBS (Hyclone, Thermo Scientific, Waltham, MA). Immediately after seeding the cells, half of the wells were inoculated with tissue culture-adapted TV (104 RNA copies per well). Cells were incubated with TV for up to 6 days before being harvested for flow cytometry and/or TV-qPCR.
Quantitative ReCV detection
For the detection of TV in fecal specimens or plasma, viral RNA was isolated from clarified 10% fecal suspensions in PBS or 100 μl of plasma using the QIAamp® Viral RNA Mini kit according to manufacturer's instructions (Qiagen GmbH, Hilden, Germany). For TV detection in cultured PBMCs, cells plus media were processed at 2 h, 24 h and 6 days PI with TV. The samples corresponding to individual wells of 24-well cell culture plate were pelleted with high-speed centrifugation (14,000 rpm) and the pellet stored in RNALater (Ambion, Austin, TX) at −20°C. The PBMCs were pelleted and washed in RNALater solution one more time before being used for RNA extraction. Total RNA was extracted using the RNeasy Plus Micro kit (Qiagen GmbH, Hilden, Germany). Precipitated RNA from both fecal specimens and PBMC cultures was eluted in 28 µl of nuclease-free water (Integrated DNA Technologies, Coralville, IA), and 8 µl of the sample was used as the template in the RT-PCR. RNA, primed with both oligo(dT) and random hexamers, was reverse-transcribed into cDNA in 20 µl reaction mixtures using Superscript™ III First-Strand Synthesis SuperMix for RT-qPCR (Invitrogen, Carlsbad, CA) according to the manufacturer's protocol. For quantitative real-time PCR, 10 µl of the cDNA product was used as the template in 50 µl reaction mixtures using Platinum Quantitative PCR SuperMix-UDG with ROX (Invitrogen) according to the manufacturer's protocol. The TV-specific primer pairs and oligonucleotide probe used were as follows: FW 5′-GAGATTGGTGTCAAAACACTCTTTG (nt position 3,645–3,669 on the TV genome, EU391643), RV 5′-ATCCAGTGGCACACACAATTT (nt position 3,820–3,800) and 6-FAM-AGTTGATTGACCTGCTGTGTCA-BHQ (nt position 3,697–3,719). PCR reactions were run in duplicate on an ABI 7900HT Fast Real-Time PCR System (Applied Biosystems, Foster City, CA) using the following amplification conditions: 2 min at 50°C, 10 min at 95°C, 40 cycles of 15 sec at 95°C, 1 min at 60°C. The threshold for detection of fluorescence above background was set at 0.185 within the exponential phase of the amplification curve. A standard curve was generated for each assay using 10-fold dilutions (from 101 to 107 copies) of a linearized plasmid containing the full TV genome. The detection limit of the assay was 10–100 copies per reaction. Negative control samples were run alongside each RNA sample from mock-infected cultures.
Human NoV detection by quantitative RT-PCR
For the detection of GII.2 and GII.4 human NoVs, viral RNA was extracted from clarified 10% fecal suspensions in PBS with the MagMaxTM -96 Viral RNA Isolation Kit (Ambion, Foster City, CA) on an automated KingFisher magnetic particle processor (Thermo Fisher Scientific, Pittsburg, PA) according to the manufacturer's instructions and eluted into 100 µl. Viral RNA was tested in a GI/GII duplex format using an AgPath-ID™ One-Step RT-PCR Kit for Probes (Applied Biosystems, Foster City, CA) on an 7,500 Realtime PCR platform (Applied Biosystems). The reaction mix of 25 µl consisted of 400 nM of each oligonucleotide primer Cog1F, Cog1R, Cog2F, and Cog2R and 200 nM of each TaqMan® Probe Ring 1C and Ring 2 [58]. Cycling conditions included reverse transcription for 10 min at 45°C, denaturation for 10 min at 95°C followed by 45 cycles of 15 sec at 95°C and 1 min at 60°C.
Nested RT-PCR for human NoV detection
Since mixtures of GII.2 and GII.4 human NoVs were used to inoculate the HB11 and GI96 macaques and RT-PCR assay was not able to differentiate between the two strains, a nested RT-PCR was designed to evaluate the strain-specific shedding in collected stool samples. Briefly, viral RNA was reverse transcribed and amplified in 20 cycles by generic primers P289/P290 in a 25 μl reaction (AccessQuick RT-PCR system, Promega, Madison, WI). One μl of the RT-PCR reaction was used as template in a nested PCR and amplified with primers 62F/63R (GTGTTGGCAGCAGCTCTAGAAATC and GTAACTTCAGAGAGCGCACAGAGA, specific for NF2003) and 64F/65R (TCATCAGAACCTCATCTGGCCCAA and AAAGGAGAACAGGGAGTTTGCCTGG, specific for NF2002) in 25 μl reactions in 35 cycles. Reactions yielded a 215 and a 225 bp product, respectively, which could be differentiated on a 2% ethidium bromide-stained agarose gel.
Flow cytometry
Cell surface marker and intracellular staining were performed as follows. PBMC cultures were harvested, low-speed centrifuged (1,300 rpm), and cell pellets were washed twice with PBS (pH 7.4) containing 0.1% sodium azide and 0.2% FBS. Fluorochrome-conjugated antibodies specific to human and/or rhesus macaque surface molecules (Table 4) as well the rhesus serum used as the primary antibody against TV, were added to cell suspensions and incubated in the dark for 30 min at RT. The cells were then washed twice with 1x Perm/Wash Buffer (BD Biosciences) and resuspended in 50 µl Perm/Wash Buffer. The permeabilized cells were stained with the primary antibody against TV for 30 min at 4°C, washed with Perm/Wash Buffer, and stained with the fluorochrome-conjugated secondary antibody (rhesus IgG-FITC, #617102012, RDI-Fitzgerald, Acton, MA) for 1 h, at 4°C. Following staining, cells were washed twice and resuspended in 300 µl of 1x BD Stabilizing Fixative (BD Biosciences). Stained and fixed cells were stored in 12×75 mm polystyrene round-bottom tubes (Becton Dickinson, Franklin Lakes, NJ) in the dark at 4°C for up to 48 h until analyzed by flow cytometry. Data were collected using the BD LSRII flow cytometer and analyzed using FACSDiva (BD Biosciences) and FlowJo software (Tree Star, Ashland, OR). A minimum of 50,000 events were collected per sample. Gating was set based on the CD3+ T lymphocyte and CD20+ B lymphocyte populations (Fig. 6A). The HLA-DR+, CD11c+, and CD123+ cell subsets within CD20+ B cell population were evaluated for the presence of TV (Fig. 7).
Statistical analysis
Statistically significant differences between proportions of TV+, HLA-DR+, CD11c+, and CD123+ cells within CD3+ and CD20+ populations of control versus TV-inoculated PBMC cultures were determined by the Student's t-test assuming equal variances. A p value of <0.05 was considered significant. Statistically significant differences between TV loads in cultured PBMCs at different time points after inoculation were also determined using the Student's t-test, with a significance level of p<0.05.
Supporting Information
Figure S1.
Duodenal biopsy from TV-negative macaque (A) and from TV-inoculated HC55 animal (B). TV antibody-specific staining shows an intense, cytoplasmic fluorescence in biopsy tissue collected at PID 3 from TV-inoculated but not from negative control animal.
https://doi.org/10.1371/journal.pone.0037973.s001
(TIFF)
Figure S2.
Individual channels (corresponding to calnexin and TV immunofluorescent staining) control data. DIC = differential interference contrast.
https://doi.org/10.1371/journal.pone.0037973.s002
(TIFF)
Acknowledgments
We thank Amanda Tardo, Surabhi Gaur, Robert Cross, Cecily Midkiff, Drs. Mostafa Bouljihad, Kaushiki Mazumdar, Pete Didier, and Preeti Chhabra for their technical assistance. We also thank Dr. Margaret K. Hostetter for her advice and support.
Author Contributions
Conceived and designed the experiments: KS TF. Performed the experiments: SF BF JD EH XA BP NG. Analyzed the data: KS SF TF JV XA BP. Contributed reagents/materials/analysis tools: JV XA BP. Wrote the paper: KS TF JV.
References
- 1. Farkas T, Sestak K, Wei C, Jiang X (2008) Characterization of a rhesus monkey calicivirus representing a new genus of Caliciviridae. J Virol 82: 5408–5416.
- 2. L'Homme Y, Sansregret R, Plante-Fortier E, Lamontagne AM, Ouardani M, et al. (2009) Genomic characterization of swine caliciviruses representing a new genus of Caliciviridae. Virus Genes 39: 66–75.
- 3. Wolf S, Reetz J, Otto P (2011) Genetic characterization of a novel calicivirus from a chicken. Arch Virol 156: 1143–1150.
- 4. Patel MM, Hall AJ, Vinjé J, Parashar UD (2009) Noroviruses: A comprehensive review. J Clin Virol 44: 1–8.
- 5. Scallan E, Hoekstra RM, Angulo FJ, Tauxe RV, Widdowson MA, et al. (2011) Foodborne illness acquired in the United States – major pathogens. Emerg Infect Dis 17: 7–15.
- 6. Atmar RL (2010) Noroviruses – State of the Art. Food Environ Virol 2: 117–126.
- 7. Zheng DP, Ando T, Fankhauser RL, Beard RS, Glass RI, et al. (2006) Norovirus classification and proposed strain nomenclature. Virology 346: 312–323.
- 8. Wyatt RG, Greenberg HB, Dalgard DW, Allen WP, Sly DL, et al. (1978) Experimental infection of chimpanzees with the Norwalk agent of epidemic viral gastroenteritis. J Med Virol 2: 89–96.
- 9. Cheetham S, Souza M, Meulia T, Grimes S, Han MG, et al. (2006) Pathogenesis of a genogroup II human norovirus in gnotobiotic pigs. J Virol 80: 10372–10381.
- 10. Rockx BH, Bogers WM, Heeney JL, van Amerongen G, Koopmans MP (2005) Experimental norovirus infections in non-human primates. J Med Virol 75: 313–320.
- 11. Souza M, Azevedo MS, Jung K, Cheetham S, Saif LJ (2008) Pathogenesis and immune responses in gnotobiotic calves after infection with the genogroup II.4-HS66 strain of human norovirus. J Virol 82: 1777–1786.
- 12. Subekti DS, Tjaniadi P, Lesmana M, McArdle J, Iskandriati D, et al. (2002) Experimental infection of Macaca nemestrina with a Toronto Norwalk-like virus of epidemic viral gastroenteritis. J Med Virol 66: 400–406.
- 13. Wobus CE, Karst SM, Thackray LB, Chang KO, Sosnovtsev SV, et al. (2004) Replication of Norovirus in cell culture reveals a tropism for dendritic cells and macrophages. PLoS Biol 2: e432.
- 14. Cannon JL, Lindesmith LC, Donaldson EF, Saxe L, Baric RS, et al. (2009) Herd immunity to GII.4 noroviruses is supported by outbreak patient sera. J Virol 83: 5363–5374.
- 15. Lindesmith L, Moe C, Lependu J, Frelinger JA, Treanor J, et al. (2005) Cellular and humoral immunity following Snow Mountain virus challenge. J Virol 79: 2900–2909.
- 16. Hutson AM, Altmar RL, Graham DY, Estes MK (2002) Norwalk virus infection and disease is associated with ABO histo-blood group type. J Infect Dis 185: 1335–1337.
- 17. Lindesmith L, Moe C, Marionneau S, Ruvoen N, Jiang X, et al. (2003) Human susceptibility and resistance to Norwalk virus infection. Nat Med 9: 548–553.
- 18. Tan M, Jiang X (2010) Norovirus gastroenteritis, carbohydrate receptors, and animal models. PLoS Pathog 6: e1000983.
- 19. Farkas T, Cross RW, Hargitt E, Lerche NW, Morrow AL, et al. (2010) Genetic diversity and histo-blood group antigen interactions of rhesus enteric caliciviruses. J Virol 84: 8617–8625.
- 20. Barron EL, Sosnovtsev SV, Bok K, Prikhodko V, Sandoval-Jaime C, et al. (2011) Diversity of murine norovirus strains isolated from asymptomatic mice of different genetic backgrounds within a single U.S. research institute. PLoS ONE 6: e21435.
- 21. Bok K, Prikhodko VG, Green KY, Sosnovtsev SV (2009) Apoptosis in murine norovirus-infected RAW264.7 cells is associated with downregulation of survivin. J Virol 83: 3647–3656.
- 22. Gerondopoulos A, Jackson T, Monaghan P, Doyle N, Roberts LO (2010) Murine norovirus-1 cell entry is mediated through a non-clathrin-, non-caveolae-, dynamin- and cholesterol-dependent pathway. J Gen Virol 91: 1428–1438.
- 23. LoBue AD, Thompson JM, Lindesmith L, Johnston RE, Baric RS (2009) Alphavirus-adjuvanted norovirus-like particle vaccines: heterologous, humoral, and mucosal immune responses protect against murine norovirus challenge. J Virol 83: 3212–3227.
- 24. LoBue AD, Lindesmith LC, Baric RS (2010) Identification of cross-reactive norovirus CD4+ T cell epitopes. J Virol 84: 8530–8538.
- 25. Perry JW, Wobus CE (2010) Endocytosis of murine norovirus 1 into murine macrophages is dependent on dynamin II and cholesterol. J Virol 84: 6163–6176.
- 26. Taube S, Perry JW, Yetming K, Patel SP, Auble H, et al. (2009) Ganglioside-linked terminal sialic acid moieties on murine macrophages function as attachment receptors for murine noroviruses. J Virol 83: 4092–4101.
- 27. Farkas T, Dufour J, Jiang X, Sestak K (2010) Detection of norovirus-, sapovirus- and rhesus enteric calicivirus-specific antibodies in captive juvenile macaques. J Gen Virol 91: 734–738.
- 28. Wei C, Farkas T, Sestak K, Jiang X (2008) Recovery of infectious virus by transfection of in vitro-generated RNA from tulane calicivirus cDNA. J Virol 82: 11429–11436.
- 29. Jiang B, McClure HM, Fankhauser RL, Monroe SS, Glass RI (2004) Prevalence of rotavirus and norovirus antibodies in non-human primates. J Med Primatol 33: 30–33.
- 30. Wang Y, Tu X, Humphrey C, McClure H, Jiang X, et al. (2007) Detection of viral agents in fecal specimens of monkeys with diarrhea. J Med Primatol 36: 101–107.
- 31. Bok K, Parra GI, Mitra T, Abente E, Shaver CK, et al. (2011) Chimpanzees as an animal model for human norovirus infection and vaccine development. Proc Natl Acad Sci U S A 108: 325–330.
- 32. Patel MM, Widdowson MA, Glass RI, Akazawa K, Vinje J, et al. (2008) Systematic literature review of role of noroviruses in sporadic gastroenteritis. Emerg Infect Dis 14: 1224–1231.
- 33. Kapikian AZ, Wyatt RG, Dolin R, Thornhill TS, Kalica AR, et al. (1972) Visualization by immune electron microscopy of a 27-nm particle associated with acute infectious nonbacterial gastroenteritis. J Virol 10: 1075–1081.
- 34. El-Kamary SS, Pasetti MF, Mendelman PM, Frey SE, Bernstein DI, et al. (2010) Adjuvanted intranasal Norwalk virus-like particle vaccine elicits antibodies and antibody-secreting cells that express homing receptors for mucosal and peripheral lymphoid tissues. J Infect Dis 202: 1649–1658.
- 35. Atmar RL, Bernstein DI, Harro CD, Al-Ibrahim MS, Chen WH, et al. (2011) Norovirus vaccine against experimental human Norwalk Virus illness. N Engl J Med 365: 2178–2187.
- 36. Smith AW, Skilling DE, Anderson MP, Benirschke K (1985) Isolation of primate calicivirus Pan paniscus type 1 from a douc langur (Pygathrix nemaeus l.). J Wildl Dis 21: 426–428.
- 37. Symes SJ, Gunesekere IC, Marshall JA, Wright PJ (2007) Norovirus mixed infections in an oyster-associated outbreak: an opportunity for recombination. Arch Virol 152: 1075–1086.
- 38. Bull RA, Tanaka MM, White PA (2007) Norovirus recombination. J Gen Virol 88: 3347–3359.
- 39. Kaplan JE, Gary GW, Baron RC, Singh N, Schonberger LB, et al. (1982) Epidemiology of Norwalk gastroenteritis and the role of Norwalk virus in outbreaks of acute nonbacterial gastroenteritis. Ann Intern Med 96: 756–761.
- 40. Yang SY, Hwang KP, Wu FT, Wu HS, Hsiung CA, et al. (2010) Epidemiology and clinical peculiarities of norovirus and rotavirus infection in hospitalized young children with acute diarrhea in Taiwan, 2009. J Microbiol Immunol Infect 43: 506–514.
- 41. Parrino TA, Schreiber DS, Trier JS, Kapikian AZ, Blacklow NR (1977) Clinical immunity in acute gastroenteritis caused by Norwalk agent. N Engl J Med 297: 86–89.
- 42. Wyatt RG, Dolin R, Blacklow NR, DuPont HL, Buscho RF, et al. (1974) Comparison of three agents of acute infectious nonbacterial gastroenteritis by cross-challenge in volunteers. J Infect Dis 129: 709–714.
- 43. Agus SG, Dolin R, Wyatt RG, Tousimis AJ, Northrup RS (1973) Acute infectious nonbacterial gastroenteritis: intestinal histopathology. Histologic and enzymatic alterations during illness produced by the Norwalk agent in man. Ann Intern Med 79: 18–25.
- 44. Dolin R, Levy AG, Wyatt RG, Thornhill TS, Gardner JD (1975) Viral gastroenteritis induced by the Hawaii agent. Jejunal histopathology and serologic response. Am J Med 59: 761–768.
- 45. Schreiber DS, Blacklow NR, Trier JS (1974) The small intestinal lesion induced by Hawaii agent acute infectious nonbacterial gastroenteritis. J Infect Dis 129: 705–708.
- 46. Otto PH, Clarke IN, Lambden PR, Salim O, Reetz J, et al. (2011) Infection of calves with bovine norovirus GIII.1 strain Jena virus: an experimental model to study the pathogenesis of norovirus infection. J Virol 85: 12013–12021.
- 47. Bailey D, Kaiser WJ, Hollinshead M, Moffat K, Chaundry Y, et al. (2010) Feline calicivirus p32, p39 and p30 proteins localize to the endoplasmic reticulum to initiate replication complex formation. J Gen Virol 91: 739–749.
- 48. Lay MK, Atmar RL, Guix S, Bharadwaj U, He H, et al. (2010) Norwalk virus does not replicate in human macrophages or dendritic cells derived from the peripheral blood of susceptible humans. Virology 406: 1–11.
- 49. Chan MC, Ho W, Sung JJ (2011) In vitro whole-virus binding of a norovirus genogroup II genotype 4 strain to cells of the lamina propria and Brunner's glands in the human duodenum. J Virol 85: 8427–8430.
- 50. Bjorck P, Kincade PW (1998) CD19+ pro-B cells can give rise to dendritic cells in vitro. J Immunol 161: 5795–5799.
- 51. Molica S, Datillo A, Mannella A, Levato D (1994) CD11c expression in B-cell chronic lymphocytic leukemia. A comparison of results obtained with different monoclonal antibodies. Haematologica 79: 452–455.
- 52. Postigo AA, Corbi AL, Sanchez-Madrid F, de Landazuri MO (1991) Regulated expression and function of CD11c/CD18 integrin on human B lymphocytes. Relation between attachment to fibrinogen and triggering of proliferation through CD11c/CD18. J Exp Med 174: 1313–1322.
- 53. Ehrhardt GR, Hijikata A, Kitamura H, Ohara O, Wang JY, et al. (2008) Discriminating gene expression profiles of memory B cell subpopulations. J Exp Med 205: 1807–1817.
- 54. Sestak K, Merritt CK, Borda J, Saylor E, Schwamberger SR, et al. (2003) Infectious agent and immune response characteristics of chronic enterocolitis in captive rhesus macaques. Infect Immun 71: 4079–86.
- 55. Sestak K, McNeal MM, Choi A, Cole MJ, Ramesh G, et al. (2004) Defining T-cell-mediated immune responses in rotavirus-infected juvenile rhesus macaques. J Virol 78: 10258–64.
- 56. Mazumdar K, Alvarez X, Borda JT, Dufour J, Martin E, et al. (2010) Visualization of transepithelial passage of the immunogenic 33-residue peptide from alpha-2 gliadin in gluten-sensitive macaques. PLoS One 5: e10228.
- 57. Ramesh G, Alvarez X, Borda JT, Aye PP, Lackner AA, et al. (2005) Visualizing cytokine-secreting cells in situ in the rhesus macaque model of chronic gut inflammation. Clin Diagn Lab Immunol 12: 192–197.
- 58. Vega E, Barclay L, Gregoricus N, Williams K, Lee D, et al. (2011) Novel surveillance network for norovirus gastroenteritis outbreaks, United States. Emerg Infect Dis 17: 1389–1395.