Epithelial cell lines of the cotton rat (Sigmodon hispidus) are highly susceptible in vitro models to zoonotic Bunya-, Rhabdo-, and Flaviviruses
© Ehlen et al. 2016
Received: 29 January 2016
Accepted: 24 April 2016
Published: 4 May 2016
Small mammals such as bats and rodents have been increasingly recognized as reservoirs of novel potentially zoonotic pathogens. However, few in vitro model systems to date allow assessment of zoonotic viruses in a relevant host context. The cotton rat (Sigmodon hispidus) is a New World rodent species that has a long-standing history as an experimental animal model due to its unique susceptibility to human viruses. Furthermore, wild cotton rats are associated with a large variety of known or potentially zoonotic pathogens.
A method for the isolation and culture of airway epithelial cell lines recently developed for bats was applied for the generation of rodent airway and renal epithelial cell lines from the cotton rat. Continuous cell lines were characterized for their epithelial properties as well as for their interferon competence. Susceptibility to members of zoonotic Bunya-, Rhabdo-, and Flaviviridae, in particular Rift Valley fever virus (RVFV), vesicular stomatitis virus (VSV), West Nile virus (WNV), and tick-borne encephalitis virus (TBEV) was tested. Furthermore, novel arthropod-derived viruses belonging to the families Bunya-, Rhabdo-, and Mesoniviridae were tested.
We successfully established airway and kidney epithelial cell lines from the cotton rat, and characterized their epithelial properties. Cells were shown to be interferon-competent. Viral infection assays showed high-titre viral replication of RVFV, VSV, WNV, and TBEV, as well as production of infectious virus particles. No viral replication was observed for novel arthropod-derived members of the Bunya-, Rhabdo-, and Mesoniviridae families in these cell lines.
In the current study, we showed that newly established cell lines from the cotton rat can serve as host-specific in vitro models for viral infection experiments. These cell lines may also serve as novel tools for virus isolation, as well as for the investigation of virus-host interactions in a relevant host species.
Infectious diseases are a major threat to human health and remain among the leading causes of death and disability worldwide . In the last decade, a variety of viruses such as Ebola virus, Hendra virus, Nipah virus, West Nile virus (WNV), and severe acute respiratory syndrome (SARS)- and Middle East respiratory syndrome (MERS)-coronaviruses have emerged or re-emerged, all of which are of zoonotic origin [2–5].
There have been a large number of novel, potentially zoonotic viruses that have been shown to be associated with small mammals, especially those of the orders Chiroptera and Rodentia, [4–14]. However, the isolation and propagation of these novel viruses has been unsuccessful in most instances, which limits further evaluation of their zoonotic risk.
Upon characterizing these novel viruses, it has become clear that most available animal models such as the domestic mouse or rat are of limited use, as they do not reflect the evolutionary conserved pathogen-host interaction that is a key trait of many reservoir-restricted viruses. In light of the large species range in which novel and potentially zoonotic viruses have been discovered, there remains a need for suitable in vitro models to understand virus-host interactions, interspecies spillover, and general viral pathogenicity . Additionally, many of the natural reservoir hosts are protected or cannot be held in captivity, which limits in vivo studies in relevant hosts. Therefore, species-specific cell culture models may serve as acceptable surrogates [16–19].
The cotton rat (Sigmodon hispidus) is a unique example of a rodent species that is a well-established animal model to study viral pathogenesis and is also associated with a large range of zoonotic viruses in the wild [20–22]. Experimental studies in cotton rats have been performed for a large variety of human viruses, including important respiratory pathogens such as influenza or parainfluenza viruses, respiratory syncytial virus, and human metapneumovirus [23–33]. Furthermore, in the wild, cotton rats are associated with a variety of known or potential zoonotic viruses, such as classical rodent-borne viruses from the genera Hantavirus and Arenavirus, as well as members of the family Flaviviridae, such as WNV and St. Louis encephalitis virus (SLEV) [34–52].
To evaluate whether the broad viral susceptibility seen in both animalmodel and wild cotton rats was also reflected in in vitro cell culture models, we generated continuous cell lines from the respiratory and renal tracts of a cotton rat, and assessed their use for virus replication studies of known and potentially novel zoonotic viruses.
Generation of epithelial cell lines
Tissues from a laboratory-bred 3-month-old male cotton rat (S. hispidus) were kindly provided by the Institute for Medical Microbiology, Immunology and Parasitology (IMMIP), University of Bonn Medical Centre, Bonn, Germany. Ethical clearance was obtained from the respective authorities (No. AZ 84-02.05.20.13.114). The trachea and both kidneys of the euthanized cotton rat where removed in toto. All subsequent steps were then performed under sterile conditions using a laminar flow hood. Briefly, organ specimens were cleaned from surrounding tissue and then either sliced or roughly chopped with a sterile blade. Tissue slices were placed in 6-well cell culture plates at 37 °C in primary cell media. For tracheal cells, airway epithelial cell growth medium was used containing the following supplements: 0.004 mL/mL bovine pituitary extract, 10 ng/mL recombinant human epidermal growth factor, 5 μg/mL recombinant human insulin, 0.5 μg/mL hydrocortisone, 0.5 μg/mL epinephrine, 6.7 ng/mL triiodo-L-thyronine, 10 μg/mL human holo-transferrin, and 0.1 ng/mL retinoic acid (Promocell, Heidelberg, Germany). For kidney cells, renal epithelial cell growth medium was used containing the following supplements: 0.05 mL/mL foetal calf serum (FCS), 10 ng/mL recombinant human epidermal growth factor, 5 μg/mL recombinant human insulin, 36 ng/mL hydrocortisone, 0.5 μg/mL epinephrine, 4 pg/mL triiodo-L-thyronine, and 5 μg/mL human holo-transferrin (Promocell). Both media were supplemented with 1 % penicillin/streptomycin (Life Technologies GmbH, Darmstadt, Germany), 0.5 % of ofloxacin (Tarivid, Sanofi-Aventis, Frankfurt, Germany) and 1 % amphotericin B (PAA, Pasching, Austria) to avoid bacterial and fungal contamination during primary cell isolation and growth.
After the outgrowth of primary cells from organ specimens, the medium was changed every 2 days, and cell outgrowth was regularly observed. When nearly confluent, cells were immortalized by lentiviral transduction of the large T antigen of SV40 as described previously [17, 19, 53]. After immortalization, cells were passaged and stock-frozen until further use. All cell cultures were genotyped by polymerase chain reaction (PCR) amplification and sequencing of the mitochondrial cytochrome c oxidase subunit I and cytochrome b oxidase subunit I genes [54, 55]. To obtain single cell clones, cells were subcloned by end-point-limiting dilution and adapted to Dulbecco’s modified Eagle’s medium (DMEM) (PAA, Cölbe, Germany) with 4.5 g/L glucose (PAA), supplemented with 10 % FCS (PAA), 2 mM L-glutamine, 1 mM sodium pyruvate (PAA), nonessential amino acids (NEAA), 1 % penicillin/streptomycin (100X concentrate contains 10,000 units/mL penicillin and 10 mg/mL streptomycin) (Life Technologies), and 1 % amphotericin B as described previously [17, 19].
Cells were seeded on glass slides, and were washed the next day with PBS and fixed with acetone-methanol (1:1) for 5 min. Then, the acetone-methanol was removed and cells were washed again with PBS. Each slide was subsequently incubated overnight at 4 °C with 250 μL primary mouse monoclonal antibodies against pan-cytokeratin (Abcam ab7753, Cambridge, UK) and rabbit polyclonal antibodies against zonula occludens-1 (ZO-1 Mid) (Invitrogen 40–2200, Carlsbad, CA, USA) diluted 1:500 in PBS. Cells were washed and then incubated for 30 min at 25 °C with 125 μL cyanine 3 (Cy3)-labelled donkey-anti-mouse and Cy2-labelled donkey-anti-rabbit secondary antibodies (Dianova, Hamburg, Germany) diluted 1:500 in PBS. Cells were washed and then nuclei were counterstained with DAPI diluted at 1:1000 in PBS for 1 min. All images were obtained with a 207 Motic AxioVision microscope (Zeiss, Jena, Germany).
Virus infection assays
Immortalized S. hispidus cells were seeded in 24-well plates at a density of 4 × 105 cells/mL and grown in DMEM containing 5 % FCS and supplements as described above. The following day, cells were infected with vesicular stomatitis virus (VSV) strain Indiana or Rift Valley fever virus (RVFV) clone 13 at multiplicity of infections (MOIs) of 0.1 and 0.001 for both viruses. Cells were infected with WNV strain New York or tick-borne encephalitis virus (TBEV) strain K23 with MOIs of 0.01 and 0.001. Infectious units of the viral stocks and in the supernatant at the end of each experiment were determined by plaque-assays with Avicel overlays for RVFV and VSV as described previously , and with agarose overlays for WNV and TBEV as described previously .
For virus infection experiments, the medium was removed and cells were inoculated with virus diluted in Optipro serum-free medium (Life Technologies) for 1 h at 37 °C. Then, cells were washed twice with PBS. Growth medium was added and supernatants were harvested 0, 12 and 24 h after infection (hpi) for VSV; 0, 24 and 48 hpi for RVFV and 0, 6, 24 and 48 hpi after infection for WNV and TBEV. All virus infection experiments were performed in three individual replicates.
Viral RNA was extracted from cell culture supernatants with the Nucleospin RNA Virus kit according to the manufacturer’s instructions (Machery-Nagel, Düren, Germany). PCR was performed using the SuperScript III One-Step RT-PCR System with Platinum Taq DNA Polymerase (Invitrogen). Cycling conditions for VSV and RVFV quantitative reverse-transcription (qRT)-PCR were as follows: reverse transcription for 15 min at 55 °C, initial denaturation for 2 min at 95 °C, and 45 cycles of denaturation for 15 s at 95 °C and primer annealing/elongation for 30 s at 58 °C. Cycling conditions for WNV qRT-PCR were as follows: reverse transcription for 30 min at 45 °C, initial denaturation for 5 min at 95 °C, and 45 cycles of denaturation for 5 s at 95 °C and primer annealing/elongation for 35 s at 57 °C. qRT-PCR was carried out using the LightCycler 480 Real-Time PCR System (Roche, Basel, Switzerland). Primers and probes are available upon request.
To test the susceptibility of the S. hispidus cell lines to a variety of novel arthropod-derived viruses, cells were seeded in 24-well plates at a density of 4 × 105 cells/mL. The following day, cells were infected with a titrated C6/36 cells-generated virus stock of Ferak , Moussa , or Cavally  virus at an MOI of 1.0. After infection, cells were observed daily for the presence of cytopathic effects (CPE). Supernatants from all infected cells were passaged onto fresh cells every 7 days for a total of three passages. Viral RNA was extracted from cell culture supernatants, and the presence of specific viral RNA was evaluated by qRT-PCR as described above.
Assessment of interferon competence
To assess the interferon (IFN) competence of the cells, cells were seeded in 24-well plates at a density of 4 × 105 cells/mL and grown in DMEM containing 10 % FCS and supplements as described above. The following day, cells were either transfected in triplicates with 1 μl of total RNA from VSV-infected cells (VSV-RNA) using the X-treme GENE siRNA transfection reagent (Roche, Basel, Switzerland) to stimulate the IFN response of the cells  or cells were left untreated as control. Eight hours after transfection, all cells were infected with the IFN-sensitive RVFV clone 13 carrying a Renilla luciferase . 16 h after infection, cells were treated with lysis buffer and Renilla luciferase activity was measured in a microplate reader.
S. hispidus and associated viruses
Viruses associated with S. hispidus as experimental animal models or natural reservoir hosts (adapted and supplemented from that of Niewiesk et al. )
Experimental animal model
Human adenovirus C
Herpes simplex virus type 1
Influenza virus A
Avian and swine influenza viruses
Influenza virus B
Respiratory syncytial virus
Human parainfluenza virus type 3
Severe acute respiratory syndrome-associated coronavirus
Human immunodeficiency virus type 1
Natural reservoir host
Whitewater Arroyo virus
Black Creek Canal virus
San Perlita virus
St. Louis encephalitis virus
West Nile virus
Cowbone Ridge virus
Vesicular stomatitis virus
Highlands J virus
Venezuelan equine encephalitis virus
Eastern equine encephalitis virus
Establishment of S. hispidus cell lines
Interferon competence of S. hispidus cell lines
Infection of S. hispidus cells with VSV and RVFV
Upon infection with RVFV at an MOI of 0.1, a maximum increase of 2.2 log in viral RNA GE copies was observed in the airway epithelial cells, and a 2.9 log increase in GE copies was seen for the renal epithelial cells. Vero E6 cells showed an increase of 2.7 log GE copies. Infections with a lower MOI of 0.001 showed comparable growth kinetics with slightly lower maximum increases in viral RNA (Fig. 3c). Production of infectious RVFV particles was assessed 48 h after infection by titration of supernatants on Vero E6 cells. The highest number of plaque-forming units was seen in ShispREC.B-6 with 6.7 log PFU/mL, followed by Vero E6 and ShispAEC.B-2 with 6.0 log and 4.5 PFU/mL after infection with an MOI of 0.1. Comparable results were observed after infection with a lower MOI resulting in 5.7; 5.1 and 3.7 log PFU/mL, respectively, for ShispREC.B-6, Vero E6 and ShispAEC.B-2 (Fig. 3d).
Infection of S. hispidus cells with WNV and TBEV
For WNV, no increase in viral RNA was seen for the airway epithelial cells at either MOI. For the renal epithelial cells, a maximum increase of viral RNA GE copies of 2.2 log was observed, and a 4.0 log increase in GE copies was seen for Vero E6 cells. Comparable growth curves were seen for the lower MOI of 0.001 Production of infectious WNV particles was assessed 48 h after infection by titration of supernatants on BHK-J cells. The highest number of plaque-forming units was seen in VeroE6 cells with approximately 6 log PFU/mL, followed by lower titers in ShispREC.B-6 with 4.0 and 4.6 PFU/mL after infection with an MOI of 0.01 and 0.001, respectively. No production of infectious particles was seen in ShispAEC.B-2 cells (Fig. 4d).
Infection of S. hispidus cells with novel insect-derived viruses
In the work presented herein, we generated epithelial cell lines from the respiratory and renal tracts of a cotton rat due to its susceptibility to a broad range of human viruses, as well as the association of multiple important and emerging zoonotic viruses with this species.
S. hispidus is a rodent species with a long-standing history as an experimental animal model for virus research. Although the first animal experiments on cotton rats date back to the 1940s, only two cell lines from cotton rats are available to date. However, in contrast to experimental animals, cell lines are a less laborious model system, less expensive, and can be used in large-scale viral experiments such as in virus isolation trials without the ethical considerations that are involved in animal experiments. From the cotton rat, an osteoblastic cell line was previously derived from an osteogenic sarcoma (CCRT), of which two lymphoid cell lines (CR-T 1 and CR-T 2) were also derived . However, these cell lines are used for the induction of tumours and as hybridoma cells to produce antibodies. No evaluation of these cells for their use in virus research has been performed despite a large range of viruses that have been investigated in S. hispidus animal experiments. Moreover, these cell lines are tumour cells that may not adequately resemble cells in vivo to study virus-host interactions, and they are not derived from target cells that are relevant to the natural course of a viral infection, such as epithelial cells. The value of species-specific cell lines has been shown particularity in the field of bat-borne viruses, where the use of bat cell lines has contributed significantly to studies of novel viruses, virus evolution, and virus adaptation during cell culture as well as replicative capacity and expression of host receptors [16, 53, 56, 63–65] (for a review see ). Cell lines derived from potential reservoir and intermediate hosts can serve as a valuable surrogate to study the replicative capacity of emerging zoonotic viruses, as has been demonstrated for the recently emerged viruses MERS-CoV and Ebola virus by work from our group [16, 56, 63, 66, 67].
In the current study, we evaluated the replicative capacity of viruses belonging to the four families Bunyaviridae, Rhabdoviridae, Flaviviridae, and Mesoniviridae in S. hispidus epithelial cell lines. Several members of the Bunyaviridae family were already shown to infect cotton rats, including Black Creek Canal virus (BCCV), which belongs to the genus Hantavirus. This virus was isolated from the lungs and spleens of cotton rats, and it was further shown by serologic analysis that S. hispidus was the primary rodent reservoir of BCCV [34, 35]. Other hantaviruses associated with S. hispidus are Bayou virus and Muleshoe virus [37, 39]. Additionally, from the genus Orthobunyavirus, an isolate termed Zegla virus was obtained from S. hispidus . Here we showed that S. hispidus epithelial cells are highly susceptible to RVFV, a bunyavirus belonging to the genus Phlebovirus, with comparable growth kinetics to interferon-deficient Vero E6 cells. Furthermore, we tested the susceptibility of S. hispidus cells to a recently isolated bunyavirus termed Ferak virus that belongs to the sister taxon of the genus Orthobunyavirus. Interestingly, no growth of this virus was seen in the S. hispidus cell lines, suggesting an insect-specific replication cycle for this virus . The further use of these cell lines for rodent-associated bunyaviruses such as hantaviruses should be evaluated in light of the promising findings for RVFV demonstrated herein.
For the Rhabdoviridae family, there have been serological findings in cotton rats that suggest a role for this species in the natural cycle of these viruses. Specifically, it was shown that neutralizing antibodies to both Indiana and New Jersey serotypes were found in S. hispidus in a VSV enzootic area in Costa Rica. Antibodies against either one or both serotypes were only found in S. hispidus, and not in exposed Mus musculus . Our in vitro results showed that VSV replicates readily in S. hispidus cell lines with high replication titres of up to almost 11 log GE copies, which is approximately only one log lower than that of the replication titres seen in Vero E6 cells. These findings suggest that the S. hispidus cell culture models could serve as suitable in vitro models for further studies on VSV. To further assess the replication capacity of other rhabdoviruses in S. hispidus cells, the insect-derived Moussa virus was used . Moussa virus was isolated from mosquitoes that also feed on mammals, but thus far, viral replication in human, hamster, or porcine cells has not been successful . However, in line with the findings of a study by Quan et al., no replication of Moussa virus was seen in our experiments with S. hispidus cells. Additionally, another insect-derived isolate of a novel virus family termed Mesoniviridae was tested on our S. hispidus cell lines. Here, no replication of Cavally virus on the newly generated cells was seen.
A strong association has been reported between the cotton rat and several zoonotic flaviviruses, including WNV, SLEV, San Perlita virus, and Cowbone Ridge virus [51, 52, 69, 70]. Furthermore, cotton rats have been discussed as potential reservoir hosts in the wild for arboviruses, by which infected viremic cotton rats serve as a reservoir for arthropods that feed on them. In our cell culture experiments with TBEV and WNV, we saw replication and production of infectious virus particles in both S. hispidus cell lines for TBEV and in the kidney epithelial cells for WNV. Moreover, both replication titres were only one log lower than that for Vero E6 cells, indicating a high susceptibility of these cell lines to flaviviruses. Additionally, we have used S. hispidus cell lines for the evaluation of a novel sylvatic isolate of SLEV in an earlier study . Here, it was shown that the endemic strain of SLEV, termed MSI-7, replicated in S. hispidus kidney cells. In contrast, the novel sylvatic SLEV isolate, termed Palenque strain, did not show any replication. As S. hispidus has been described as a natural reservoir host for SLEV, these findings suggest that the sylvatic isolate has not yet adapted to hosts that live outside the primary rain forest, whereas the endemic strain has . In line with the findings obtained for SLEV, our results showed that WNV only replicated in kidney cells but not in airway epithelial cells, suggesting that kidney cells are more susceptible to this virus than airway cells. Taken together, the multiple in vitro findings presented herein for flaviviruses provide evidence that cotton rats may be reservoirs for multiple members of Flaviviridae in the wild. Therefore, S. hispidus cell lines, especially S. hispidus kidney epithelial cells, may provide a useful model for in vitro virus-host interaction studies.
Newly generated epithelial cell lines from S. hispidus are able to support the replication of virus species from important zoonotic virus families, and may therefore serve as valuable tools for studies focusing on the isolation of novel viruses and virus-host interactions.
We thank Marco Marklewitz, Pascal Trippner and Anne Kopp for help with novel arthropod-derived viruses; Beate Kümmerer and Janett Wieseler for viral isolates of WNV and TBEV; and Bettina Dubben for organ samples. We thank Friedemann Weber (University of Gießen) for providing RVFV clone 13 and RVFV-Renilla reporter virus and Alexander Pfeifer, (University of Bonn) for providing large T antigen lentiviruses.
The work was funded by the German Research Platform for Zoonoses and the Federal Ministry of Education and Research (Grant No. 01KI1308 to IE).
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