Volume 11, Number 4—April 2005
Experimental Infection of Prairie Dogs with Monkeypox Virus
Studies of experimental infection of prairie dogs (Cynomys ludovicianus) with monkeypox virus are described. After intraperitoneal infection, all of the animals died within 11 days. Virus was cultured from their blood and oropharynx several days before death; at necropsy, most of the organs tested contained monkeypox virus. Marked hepatic and splenic necrosis were observed, along with mild inflammatory changes in the lungs. After intranasal infection, the primary pathologic changes were in the lungs and pleural cavity. Some of the intranasally infected animals (40%) survived, and monkeypox virus could be cultured from their nasal discharge and oropharynx for <22 days. Ulcerative lesions also developed on the lips, tongue, and buccal mucosa of the surviving animals. Our findings support an earlier report, which suggested that infected prairie dogs can transmit monkeypox virus by respiratory and mucocutaneous contact with susceptible animals and persons.
In the summer of 2003, an outbreak of monkeypox virus infection occurred among humans living in the midwestern United States (1,2). A total of 32 human cases were confirmed. Most of the patients experienced a brief febrile illness with vesicular skin eruptions; no deaths resulted. Most patients with this illness had a history of contact with sick pet prairie dogs (Cynomys spp.), originally obtained from a single pet distributor (1,2). The epidemiologic investigation, clinical findings, and control of this outbreak were described (1).
A recent publication (2) reported the pathologic findings at necropsy in 2 sick prairie dogs confiscated during the 2003 outbreak. The animals showed necrotizing bronchopneumonia, conjunctivitis, and tongue ulceration. Virus isolation and electron microscopy examination of tissue samples from the animals demonstrated active viral replication in lungs and tongue, which suggested that both respiratory and mucocutaneous exposures are potentially important routes of monkeypox virus transmission from rodents to humans. To learn more about the nature of monkeypox virus infection in prairie dogs, we experimentally infected 10 of the animals with a human isolate from the 2003 U.S. outbreak.
Ten wild-caught, adult prairie dogs (Cynomys ludovicianus) were obtained from a commercial trapper, with permission of the Food and Drug Administration. Animals were housed in pairs in large (61 cm × 61 cm × 45 cm) metal cages within a Duo-Flow biosafety cabinet (Biochem Lab Products, Seaford, DE, USA) in an isolation room of an animal biosafety level 3 facility. All persons handling the animals had recently received a smallpox (vaccinia) vaccination and used appropriate personal protection. Animals were cared for in accordance with the guidelines of the Committee on Care and Use of Laboratory Animals (Institute of Laboratory Animal Resources, National Research Council) under an animal use protocol approved by the Institutional Animal Care and Use Committee at the University of Texas Medical Branch.
The strain of monkeypox virus used (provided by the Centers for Disease Control and Prevention, Atlanta, Georgia, USA) was designated MPX 2003. This virus was originally isolated from a skin lesion of a person with monkeypox during the 2003 outbreak in the United States (1). A stock of the virus was prepared from infected Vero cells and was used to infect the rodents; the unsonicated frozen cell lysate had a titer of 106.1 PFU/mL.
Tissues and other samples for virus assay were stored at –80°C. For analysis, the tissue samples were thawed and triturated in sterile TenBroeck glass tissue grinders in phosphate-buffered saline (PBS), pH 7.4, containing 30% heat-inactivated (56°C for 30 min) fetal bovine serum (FBS) to prepare a 10% tissue homogenate. After centrifugation at 5,000 rpm for 5 min to clarify the suspension, serial 10-fold dilutions from 10–1 to 10–8 were prepared in PBS containing 10% FBS. Similar dilutions were made with blood and throat swab suspensions for virus assay.
Dilutions of the tissue homogenates, blood, and throat swab suspensions were titrated in 24-well cultures of Vero cells, 4 wells per dilution, as described before (3). Cultures were incubated at 37°C, and plaques were counted 6 days later, as they were sharp and easy to read at that time. Virus titers were defined as the log of PFU per milliliter of sample.
Experimental Infection of Animals
Since the response of prairie dogs to monkeypox virus infection was uncertain when these experiments were conducted, the animals were infected by the intraperitoneal (IP) or intranasal routes. Four rodents (MPX-1 to MPX-4) were injected IP with 105.1 PFU of MPX 2003 virus. The other 6 animals (MPX-5 to MPX-10) were infected by the intranasal route; under Halothane (Halocarbon Laboratories, River Edge, NJ, USA) anesthesia, 2 drops (≈100 μL) of the stock virus solution containing 106.1 PFU/mL were instilled into each nostril. After infection, all rodents were observed daily for signs of illness; if an animal died, a necropsy was performed, and tissues (liver, spleen, kidney, adrenal, pancreas, lung, heart, and brain) were taken for histopathologic examination and virus titration. Blood (100 μL from the retroorbital sinus) and an oropharyngeal swab were also taken daily from each animal for virus assay. The whole blood and the swab were expressed in 900 μL of PBS with 10% FBS. Twenty-five days after infection, the surviving animals were exsanguinated and euthanized, and a necropsy was performed to obtain tissue samples.
Complement fixation (CF) tests were performed by microtechnique (4) with 2 full units of guinea pig complement and antigen titers >1:32. The antigen used in the CF tests was prepared from brains of infected baby mice injected intracerebrally with vaccinia virus; infected brains were treated by the sucrose acetone extraction method (4). CF antibody titers were recorded as the highest serum dilution giving +3 or +4 fixation of complement.
Plaque reduction neutralization (PRN) tests were conducted in 24-well microplate cultures of Vero cells, by using a technique described previously (5). The MPX 2003 virus was used at a dose of ≈20 PFU. Serial 10-fold dilutions of each serum specimen were incubated overnight at 5°C with the virus dose, before inoculation. Plaques were read on day 6 after inoculation; a 50% reduction of virus plaques, compared to uninfected control prairie dog serum, was used as the endpoint (6). PRN antibody titers were recorded as the highest serum dilution that produced >50% plaque reduction.
Histopathologic and Immunohistochemical Methods
At necropsy, tissue samples were taken from the animals and preserved in 10% buffered formalin for 24 to 48 h, followed by storage in 70% ethanol. After fixation, the samples were processed for routine embedding in paraffin. Four- to 5-μm-thick tissue sections were made and stained by the hematoxylin and eosin (H&E) method (5).
Selected tissue sections were also studied immunohistochemically, by using vaccinia hyperimmune mouse ascitic fluid (1:100 dilution) as the primary antibody. A mouse-on-mouse IHC-ISO labeling kit (InnoGenex, San Ramon, CA, USA) was used, according to the manufacturer’s instructions and a published protocol (7). The primary antibody was incubated with the sections at 4°C overnight. Tissue sections from an uninfected animal were used as negative controls.
Two animals, MPX-2 and MPX-10, died of respiratory arrest during anesthesia and sample collection on days 5 and 6, respectively. They were omitted from the results.
Beginning on approximately day 4 after infection, most of the prairie dogs became lethargic and anorexic. The 3 animals that were infected IP (MPX-1, MPX-3, and MPX-4) died 8–11 days after infection. Visible lesions did not develop on the skin or mucous membrane of any of these animals.
Three of 5 intranasally infected animals (MPX-6, MPX-7, and MPX-9) also died; their deaths occurred 11–14 days after infection. Their clinical symptoms (increasing lethargy and anorexia) were the same as those observed in the IP infected group. Two of the intranasally infected prairie dogs (MPX-5 and MPX-8) survived infection, although they were lethargic and anorexic for several days between weeks 1 and 2 after infection. In the latter 2 animals, vesicular lesions developed on their lips and tongue, along with nasal congestion and a mucopurulent nasal discharge. Inoculation of fresh samples of the nasal discharge into Vero cell cultures yielded monkeypox virus; and smears of the discharge, stained by immunofluorescence with a vaccinia hyperimmune mouse ascitic fluid, demonstrated swollen macrophages containing multiple fluorescent inclusion bodies, characteristic of poxvirus infection (Figure 1). The nasal congestion and discharge continued for ≈10 to 14 days, but it gradually diminished, and the 2 surviving prairie dogs appeared healthy when they were euthanized 25 days after infection.
In the IP infected group (MPX-1, MPX-3, and MPX-4), monkeypox virus was first detected simultaneously in the blood and throat on day 5 or 6 after infection (Table 1). The amount of virus in these samples increased daily until death. In the IP infected group, the highest virus titers were found in liver and spleen; lower titers were observed in kidney and lung (Table 2).
The temporal appearance, organ distribution, and amount of virus present in the blood, throat, and tissues of the intranasally infected prairie dogs were quite different. Among the 3 animals with fatal infections (MPX-6, MPX-7, and MPX-9) in this group, monkeypox virus appeared in the throat several days before it was detected in the blood (Table 1). At death, animal MPX-9 had 108.0 PFU/g of virus in lung; smaller amounts of virus were detected in liver, spleen, kidney, and heart (Table 2). In contrast, no virus could be detected in these same organs in animals MPX-6 or MPX-7 at death.
Likewise, monkeypox virus was detected in the throats of the 2 surviving animals (MPX-5 and MPX-8) for 19 and 22 consecutive days, respectively (Table 1). No samples were taken on day 24; but throat swabs taken from MPX-5 on days 23 and 25 were negative; and samples from MPX-8 were negative on day 23 but positive (100.7) on day 25 (data not shown). In these 2 animals, a comparable level of viremia developed; but the duration was uncertain, since no blood samples were taken after day 15. However, blood and organ cultures from the 2 survivors were negative when they were euthanized and underwent necropsy 25 days after infection (Table 2).
All of the blood samples taken from the infected prairie dogs (Table 1) were examined by CF test for monkeypox virus antibodies, by using a vaccinia antigen. Only 2 samples gave a positive reaction. Blood (serum) samples from the 2 survivors, MPX-5 and MPX-8, both had a CF antibody titer of 1:64 on day 25 after infection, when the animals were euthanized. The last previous blood samples from these animals were taken on day 15 and were negative, so seroconversion occurred during week 2 or 3 after infection.
Serum specimens from MPX-5 and MPX-8, collected 25 days after infection, were also tested by PRN. Using 50% plaque inhibition as an endpoint, both animals had a neutralizing antibody titer of 1:320 against monkeypox virus.
No histologic abnormalities were noted in the heart, pancreas, kidneys, or adrenal glands of any of the animals, regardless of the route of infection. The gastrointestinal tracts of a few animals were examined and were likewise unremarkable.
Animals Infected Intraperitoneally
At necropsy, firm nodular changes were observed in the abdominal adipose tissue (omentum) of the animals in this group (MPX-1, MPX-3, and MPX-4). Microscopically, multifocal necrosis of adipose tissue occurred, with vasculitis, prominent fibroblast proliferation, and infiltration by macrophages and other inflammatory cells (Figure 2A). Their spleens showed moderate to severe necrosis, mainly in the lymphoid areas as described before (3). The livers showed centrilobular necrosis, with some inflammatory cellular infiltration and prominent inclusion bodies in the hepatocytes (Figure 2B). The lungs exhibited mild-to-moderate thickening of the interstitium, with increased infiltration by mononuclear inflammatory cells.
Animals Infected Intranasally
No evident hepatic lesions or splenic necrosis was observed in the 5 animals infected intranasally (MPX-5 to MPX-9). One of the animals (MPX-9) had marked inflammation and necrosis of adipose tissue and skeletal muscle, with proliferation of large fibroblasts and macrophages. The mediastinal lymph nodes, and thymus in some animals, exhibited marked lymphoid necrosis and depletion, with the infiltration by plump inflammatory cells containing dense eosinophilic material (Figure 2C). The lungs of animals MPX-6, MPX-7, and MPX-9 showed marked edema, hemorrhage, and necrosis, which also involved the pleura and muscle of the diaphragm. Extensive adhesions and a proliferation of swollen cells containing globules of eosinophilic material, later shown by immunohistochemical tests to be viral antigen, were evident in these structures (Figure 2D).
The 2 surviving animals in this group (MPX-5 and MPX-8) were euthanized on day 25 in apparent good health. Few histologic abnormalities were noted at necropsy, except for focal inflammation in the skin (lymphocytic infiltration in dermis). An immunostain of the skin for viral antigen was negative. Animal MPX-8 also had multifocal inflammation of the lung with epithelial and giant cell granulomas.
Selected tissue sections were studied immunohistochemically (IHC), by using a vaccinia mouse hyperimmune mouse and an IHC-ISO labeling kit. Tissue sections from 2 uninfected prairie dogs were used as negative controls. No positive staining was observed in the control animals. Likewise, tissues from the 2 survivors (MPX-5 and MPX-8) were also IHC-negative.
Animals Infected Intraperitoneally
In the liver of IP infected animals (MPX-1, MPX-3, and MPX-4), most of the inclusion bodies were strongly IHC-positive for poxvirus antigen. Depending on the severity of the histologic abnormality, this positive staining sometimes involved the surrounding cytoplasm and cellular membranes. Some of the smaller inclusion bodies were negative. The spleen was also IHC-positive, corresponding to the severity of pathologic changes. In some animals, the cells lining the surface of the splenic capsule (mesothelial cells) were enlarged or tall and stained strongly positive for viral antigen. In these animals, the positive staining also appeared to involve the superficial zones of the neighboring organs such as the pancreas and adrenals, which were otherwise negative and without pathologic changes. This pattern suggested direct virus spread between adjacent sites when the boundaries (capsules) were broken. Necrotic areas in the perisplenic and periadrenal fat also stained strongly positive.
Animals Infected Intranasally
In animal MPX-9, viral antigen was present in the liver, lungs, mediastinum, and bronchus. The mediastinal lymph nodes were also strongly positive, accompanied by central necrosis. An antigen-positive area in a bronchus of this animal showed distinctive epithelial cell proliferation and squamous metaplasia, as opposed to a negative zone, which was lined by normal columnar epithelium (Figure 3).
Although no evidence of hepatocytic degeneration or necrosis was seen in the H&E-stained sections of liver from the other 4 animals in this group (MPX-5 to MPX-8), the immunostain for viral antigen highlighted rare inclusion bodies in the hepatocytes of animals MPX-6 and MPX-7, which indicated a small amount of monkeypox virus replication in the liver. The spleens of these 4 animals were negative for monkeypox virus antigen by IHC. Scattered antigen-positive interstitial cells (mostly macrophages) were observed in lungs of animal MPX-6; but lungs in the other animals (MPX-5, MPX-7, and MPX-8) were negative by IHC. Sections of the adrenals, kidneys, and heart of all of the infected animals were likewise negative.
Results of this study confirm that prairie dogs are highly susceptible to infection with monkeypox virus, although the observed death rate and pathologic changes were less severe than in 13-lined ground squirrels (Spermophilus tridecemlineatus) that had been infected IP and intranasally with the same virus dose (3). In contrast to ground squirrels, the pathogenesis and severity of monkeypox virus infection in prairie dogs varied, depending on the route of infection. The IP infected prairie dogs all died after infection; at necropsy, marked hepatic and splenic necrosis was seen, along with mild-to-moderate inflammatory changes in the lungs. Only 3 of the 5 intranasally infected prairie dogs died. In 1 of these animals (MPX-9), the virologic, histopathologic, and immunohistochemical findings were similar to those observed in the IP infected prairie dogs. However, in the other 2 animals with fatal infections (MPX-6 and MPX-7), few pathologic changes were observed in the liver, spleen, or other abdominal organs, although marked edema, hemorrhage, and necrosis were observed in the lungs. The reason for this different response is unknown, but our sample size was small.
The pattern of monkeypox virus infection seen in the 2 surviving prairie dogs (MPX-5 and MPX-8) was potentially the most important. These 2 animals continued to have infectious monkeypox virus in their throat and nasal discharge for several weeks after infection.
The pattern of experimental infection in the intranasal group of prairie dogs concurs with the clinical and pathologic observations made during the 2003 monkeypox virus outbreak in the United States. Guarner et al. (2) reported that 10 (67%) of 15 prairie dogs in 1 affected pet store died rapidly; the other 5 animals exhibited anorexia, wasting, sneezing, coughing, swollen eyelids, and nasal discharge. Our intranasally infected animals manifested similar symptoms and had a comparable death rate (60%). Two of the sick prairie dogs at the affected pet store were euthanized, and necropsies were performed (2).
Apart from ulcerative lesions on the tongue and eyelids, these animals had bronchoalveolar pneumonia with edema, necrosis, and a marked infiltrate of macrophages containing many poxvirus particles. Mild inflammatory changes occurred in the liver and spleen, and other organs appeared normal. Although direct culture of monkeypox virus from tissues of these 2 animals was not attempted, the authors noted difficulty detecting monkeypox virus DNA by standard polymerase chain reaction (PCR) and by PCR followed by restriction-endonuclease fragment length polymorphism, even though viral antigen was easily detected by IHC in the same tissue samples (2).
Our experience was similar with animals MPX-6 and MPX-7. Despite the presence of viral antigen in the liver of these 2 experimentally infected prairie dogs, cultures of their lungs, livers, and spleens did not yield infectious virus. Yet on the day before death, monkeypox virus was isolated from their blood and throat swabs. Thus the exact cause of death in these 2 animals is uncertain.
In animals MPX-5 and MPX-8, cutaneous ulcerative lesions developed on the lips, tongue, and buccal mucosa, along with nasal congestion and discharge. The same clinical manifestations were reported from the affected pet prairie dogs (2). In view of the prolonged shedding of monkeypox virus in the throat and nasal discharge of animals MPX-5 and MPX-8, such pets likely could easily transmit virus by direct contact or by bite to cagemates or to humans handling them. Guarner et al. (2) concluded that both respiratory and direct mucocutaneous exposures are potentially important routes of transmission of monkeypox virus between rodents and humans. Our findings with experimentally infected prairie dogs support those conclusions.
Dr. Xiao is associate professor in the Department of Pathology at the University of Texas Medical Branch, where he is also a member of the Center for Biodefense and Emerging Infectious Diseases.
We are grateful to Inger K. Damon for providing monkeypox virus, Dora Salinas for helping prepare the manuscript, and Patrick Newman and Mengyi Ye for assisting in tissue processing and immunohistochemical staining.
This work was supported by contract NO1-AI25489, NO1-AI30027, and U54-AI57156 from the National Institutes of Health.
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