Skip directly to site content Skip directly to page options Skip directly to A-Z link Skip directly to A-Z link Skip directly to A-Z link
Volume 24, Number 9—September 2018
Research

Novel Orthopoxvirus and Lethal Disease in Cat, Italy

On This Page
Materials and Methods
Results
Discussion
Cite This Article
Figures
Figure 1
Figure 2
Figure 3
Tables
Table 1
Table 2
Downloads
Article
RIS [TXT - 2 KB]
Article Metrics
Metric Details
18
citations of this article
EID Journal Metrics on Scopus
Author affiliations: University of Bari, Valenzano, Italy (G. Lanave, G. Dowgier, N. Decaro, M. Losurdo, V. Martella, C. Buonavoglia, G. Elia); La Vallonea Veterinary Laboratory, Milan, Italy (F. Albanese); Centro Veterinario Montarioso, Siena, Italy (E. Brogi); Istituto Zooprofilattico Sperimentale di Puglia e Basilicata, Putignano, Italy (A. Parisi); Istituto Zooprofilattico Sperimentale di Lombardia ed Emilia Romagna, Brescia, Italy (A. Lavazza)

Cite This Article

Abstract

We report detection and full-genome characterization of a novel orthopoxvirus (OPXV) responsible for a fatal infection in a cat. The virus induced skin lesions histologically characterized by leukocyte infiltration and eosinophilic cytoplasmic inclusions. Different PCR approaches were unable to assign the virus to a defined OPXV species. Large amounts of typical brick-shaped virions, morphologically related to OPXV, were observed by electron microscopy. This OPXV strain (Italy_09/17) was isolated on cell cultures and embryonated eggs. Phylogenetic analysis of 9 concatenated genes showed that this virus was distantly related to cowpox virus, more closely related to to ectromelia virus, and belonged to the same cluster of an OPXV recently isolated from captive macaques in Italy. Extensive epidemiologic surveillance in cats and rodents will assess whether cats are incidental hosts and rodents are the main reservoir of the virus. The zoonotic potential of this novel virus also deserves further investigation.

Orthopoxviruses (OPXVs; family Poxviridae, subfamily Chordopoxvirinae, genus Orthopoxvirus) are complex, double-stranded DNA viruses with ongoing interest because of their potential use as bioterrorism agents and in gene therapy. Variola virus (VARV), the causative agent of smallpox, has been eradicated in nature; however, there is still the possibility of accidental or intentional release, and it is currently classified as a category A biologic agent (1). Another concern is the zoonotic potential of some OPXVs, such as monkeypox virus, camelpox virus, buffalopox virus, and cowpox virus (CPXV) (2,3).

CPXV, which has a wide host range and a distribution restricted to the Eurasian continent, causes localized dermatitis in humans, although severe disease might develop in immunocompromised persons, occasionally with a fatal outcome. Natural hosts for CPXV are wild rodents (4), but the infection is acquired mainly through direct contact with cats, which are natural hosts, and rarely by exotic animals and wild species (5). Ectromelia virus (ECTV) is the causative agent of mousepox, a severe exanthematous disease of mice in laboratory colonies and has been reported worldwide in several outbreaks and causes high economic losses in biomedical research (6). ECTV has never been reported in humans, and little is known regarding its natural distribution and hosts (7).

Reports of OPXV infections in animals and humans have largely increased during recent decades, which has enhanced their zoonotic potential and led to the perception of an increasing risk for humans (8). For cats, there are several reports of poxvirus infections, but the causative agent has been characterized as CPXV (9–14) or has not been characterized (15–18).

We report a case of fatal infection with an OXPV in a household cat. This virus was more closely related to ECTV than to CPXV, putatively representing a novel OPXV species.

Materials and Methods

Case Study

Figure 1

Thumbnail of Cat with orthopoxvirus infection, Italy. Nodular skin lesions were observed on the snout (A), thorax (B), and forelimb (C). Skin punch biopsy specimen (D) showing leukocyte infiltration and cytoplasmic inclusion bodies (arrows) (hematoxylin and eosin stain, original magnification ×100).

Figure 1. Cat with orthopoxvirus infection, Italy. Ulcerated nodules and plaques were observed on the lips (A), thorax (B), and forelimb (C). Skin punch biopsy specimen (D) showing leukocyte infiltration and cytoplasmic inclusion...

A domestic, short-haired, male, 6-month-old cat was brought to a veterinarian because of multicentric, nodular, ulcerative dermatitis (Figure 1). The cat was regularly vaccinated for common feline diseases (feline panleukopenia, rhinhotracheitis, calicivirosis, and chlamydiosis) and showed negative test results for retroviral infections. An antiparasitic product had been applied monthly (Frontline Combo Spot On; Merial, Ingelheim, Germany). The cat was fed a balanced commercial diet and lived indoors, but it had access to outdoors and had a hunting behavior.

The cat had multiple nodular, plaque-like, ulcerative lesions on its body, particularly on the feet and face. Results of diagnostic testing, including a wood lamp examination, skin scrapings, trichogram, and fungal culture, were negative. Cytological examination showed a mixed inflammatory population of cells with a relevant amount of eosinophils. A blood test showed only a mild leukocytosis with an increase in numbers of lymphocytes, neutrophils, and eosinophils. Because of rapid worsening of its clinical conditions, the cat was euthanized.

Histopathologic Analysis

We collected multiple skin biopsy specimens for histopathologic analysis by using an 8-mm biopsy punch and fixed these specimens in 10% buffered formalin. Samples were embedded in paraffin, sectioned, and stained with hematoxylin and eosin, according to standard protocols.

DNA Extraction and PCR Amplification

An OPXV infection was suspected on the basis of clinical presentation and histopathologic analysis. Therefore, we processed histologic preparations for molecular investigations to confirm the presumptive diagnosis. We purified total DNA from a thin section of ≈20 mg of formalin-fixed, paraffin-embedded tissue by using the DNeasy Blood and Tissue Kit (QIAGEN, Hilden, Germany) according to the manufacturer’s instructions.

We tested the DNA extract by using 2 panchordopoxvirus PCRs specific for the variable GC content of the genera included in the subfamily Chordopoxvirinae and other unclassified chordopoxviruses (19). For the low GC content PCR, we used DNA from a laboratory vaccinia virus Western Reserve strain (VACV-WR) as a positive control. For the high GC content PCR, we used an Orf virus isolated during an outbreak of contagious ecthyma as a positive control. We initially conducted subsequent identification of OPXV by using a PCR specific for the gene coding A-type inclusion protein (20), followed by a second PCR specific for the hemagglutinin (HA) gene (21). In addition, we performed 2 species-specific PCRs, 1 for ECTV and 1 for CPXV, to further characterize the virus (22).

We conducted all PCR amplifications by using an LA PCR Kit (version r.2.1) (Takara Bio, Tokyo, Japan) in a 50-μL reaction containing 1 mmol/L of primers, LA PCR Buffer (Mg2+), 8 μL of dNTP mixture (corresponding to 400 mmol/L of each dNTP), 2.5 units of TaKaRa LA Taq polymerase, and 1 μL of template DNA. The cycling protocol used for each assay was programmed as described (19). PCR products were subjected to electrophoresis on a 1.5% agarose gel containing a fluorescent nucleic acid marker (GelRed; Bio-Rad Laboratories, Hercules, CA, USA) at 80 V for 45 min and visualized under fluorescent light on the Gel Doc EZ Imaging System with Image Laboratory Software (Bio-Rad Laboratories). PCR products were directly sequenced by Eurofins Genomics GmbH (Ebersberg, Germany). We manually edited and analyzed sequences by using the Geneious platform version 10.1.3 (Biomatters Ltd., Auckland, New Zealand).

Virus Isolation

After diagnosis of OPXV infection, we collected additional biopsy specimens from skin lesions of the diseased cat intravitam and used them for subsequent virologic investigations. For virus isolation, we used African green monkey kidney fibroblast CV-1 cells and African green monkey kidney epithelial Vero cells. Cells were grown in Dulbecco’s modified minimum essential medium (DMEM) supplemented with 10% fetal bovine serum. Tissues were homogenized in DMEM (10%, wt/vol) and centrifuged at 8,000 × g for 10 min. Supernatants were treated with antimicrobial drugs (penicillin 5,000 IU/mL, streptomycin 2,500 μg/mL, and amphotericin B 10 μg/mL) for 30 min, inoculated on partially confluent CV-1 and Vero cell cultures, and incubated at 37°C in a 5% CO2 incubator. After an adsorption period of 45 min, DMEM was added. Cells were observed daily for cytopathic effects.

For hematoxylin and eosin staining and indirect immunofluorescence (IIF) assay, we grew cells on coverslips placed in 12-well plates. Cells were mock- or virus-infected and coverslips were harvested at 48 hours postinfection. For detection of inclusion bodies, we fixed cells in Bouin solution for 2 h and stained them with hematoxylin and eosin. For the IIF assay, cells were fixed with 80% acetone for 30 min. Coverslips were rinsed twice with phosphate-buffered saline and incubated 30 min in a humidified chamber at 37°C with a serum sample (diluted 1:50) collected from the ill cat. Coverslips were washed twice with phosphate-buffered saline and incubated with goat anti-cat IgG conjugated with fluorescein isothiocyanate (Sigma-Aldrich, Milan, Italy).

The homogenate of skin biopsy specimens was inoculated onto the chorioallantoic membrane of 12-day-old chick embryos. After 2 days of incubation at 37°C, membranes were collected from the eggs and pock morphology was observed.

Electron Microscopy

We performed negative staining and electron microscopic analysis of homogenates of skin punch biopsy specimens and supernatants of infected Vero cells that showed an evident cytopathic effect. Samples were frozen and thawed twice and centrifuged at 4,000 × g for 20 min and at 9,300 × g for 10 min to clarify the supernatant. The second supernatant (82 μL) was then ultracentrifuged in an Airfuge centrifuge (Beckman Coulter, Brea, CA, USA) for 15 min at 21 lbs/in2 (82,000 × g). The Airfuge was fitted with an A 100 rotor that held six 175-μL test tubes containing specific adapters for 3-mm grids, which enables direct pelleting of virus particles on carbon-coated, formvar copper grids. These grids were stained with 2% sodium phosphotungstate, pH 6.8, for 1.5 min, and observed with a Tecnai G2 Biotwin Transmission Electron Microscope (Field Electron and Ion Company, Hillsboro, OR, USA) operating at 85 kV. We identified poxvirus particles, observed at magnifications of 11,000×–26,500×, on the basis of their typical morphologic characteristics.

Serologic Analysis

We tested the serum sample collected intravitam from the diseased cat for OPXV antibodies by virus neutralization and IIF assays. We used strains Italy_09/17 isolated from the same cat and VACV-WR in these tests.

For the virus neutralization test, we mixed 2-fold dilutions of heat-inactivated serum (starting at a dilution of 1:2) with 100 50% tissue culture infective doses of virus in 96-well microtiter plates. After incubation at room temperature for 60 min, 2 × 104 CV-1 cells were added to each well. Plates were read after 4 days of incubation at 37°C in a humidified atmosphere of 5% CO2.

For the IIF assay, we fixed confluent monolayers of CV-1 cells grown on coverslips and infected with strain Italy_09/17 or VACV-WR with 80% acetone. We tested 2-fold dilutions of heat-inactivated serum (diluted 1:20 to 1:5,120) by using 1 coverslip/dilution. Goat anti-cat IgG conjugated with fluorescein isothiocyanate was used as a secondary antibody (Sigma-Aldrich).

Next-Generation Sequencing

For DNA extraction, we obtained virus stocks from semipurified virus particles. In brief, we infected CV-1 cells with strain Italy_09/17. At 48 hours postinfection, the cell medium was collected and nuclei and cell debris were discarded by centrifugation at 1,000 × g for 10 min at 4°C. We extracted virus DNA by using a QIAamp Cador Pathogen Mini Kit (QIAGEN) according to the manufacturer’s instructions.

We quantified DNA by using the Fluorometric Qubit dsDNA High Sensitivity Assay Kit (Thermo Fisher Scientific, Waltham, MA, USA). We prepared a genomic DNA library by using the Nextera DNA Sample Prep Kit (Illumina, San Diego, CA, USA) according to the manufacturer’s protocol and performed a size-selection step manually by using Ampure XP magnetic beads (Beckman Coulter). We performed quality control analysis of the sample library by using the QIAxcel Advanced System with QIAxcel ScreenGel Software 1.4.0 (QIAGEN). We normalized library samples as suggested by QIAGEN and performed sequencing by using a MiSeq instrument, version 2, and a MiSeq Reagent Kit (Illumina).

Genome Annotation and Comparison

We obtained 1,497,762 paired reads in next-generation sequencing (NGS) experiments (Illumina); these reads had an average length of 155.4 bp. We performed quality control of reads by using FastQC (23) and sequence trimming by using the plugin Trim Ends in Geneious software version 10.1.3 (https://www.geneious.com/). We filtered NGS sequences by using the genome of African green monkey (Chlorocebus sabeus), which yielded 217,236 unmapped reads. We used these unmapped reads for de novo assembling of the feline OPXV genome by using the Geneious Assembler.

We annotated the nearly full-length genome sequence of the Italy_09/17 isolate by using ECTV strain Naval as reference (GenBank accession no. KJ563295). We performed genome annotation by using FindORFs software in Geneious version 10.1.3 and a set of reference sequences, including ECTV Naval (accession no. KJ563295), ECTV Mos (accession no. AF012825), CPXV BR (accession no. AF482758), and VACV COP (accession no. 35027) for comparison. We further analyzed open reading frames that remained unassigned or with a lower similarity to the reference sequences by using MyOrfeome (http://myorfeome.sourceforge.net).

Phylogenetic Analysis

For characterization of the OPXV strain, we used the strategy proposed by Emerson et al. (24). We selected 9 coding sequences from the genome of the feline OPXV strain Italy_09/17: A7L, early transcription factor/VETF large subunit; A10L, major core protein; A24R, RNA polymerase 132; D1R, messenger RNA capping enzyme, large subunit; D5R, DNA-independent NTPase (DNA replication); E6R, hypothetical protein; E9L, DNA polymerase; H4L, RNA polymerase-associated protein; and J6R, RNA polymerase 147. Gene designations refer to the VACV COP genome. We aligned concatenated genome sequences of OPXVs representative of North American and Old World (African and Eurasian) viruses by using Geneious version 10.1.3 and the MAFFT algorithm (25). After searching the GenBank database, we retrieved complete HA gene sequences of 2 feline-derived human OPXV strains (accession nos. EF612709 and FJ445747) and of an OPXV isolated from captive macaques (accession no. KY100116) and aligned them with cognate OPXV sequences.

We performed phylogenetic analysis for concatenated DNA alignments with Bayesian inference by using 4 chains run for >1 million generations (26,27). We used ModelTest software (http://evomics.org/resources/software/molecular-evolution-software/modeltest/) to identify the most appropriate model of evolution for the entire dataset and for each gene individually. The identified program settings for all partitions, under the Akaike Information Criteria, included 6 character states (general time reversible model), a proportion of invariable sites, and a gamma distribution of rate variation across sites. We deposited nucleotide sequences of strain Italy_09/17 used for phylogeny in GenBank (accession nos. MF578930–9).

Detection of Other Pathogens

We subjected nucleic acids extracted from freshly collected skin biopsy specimens and serum of the affected cat to a TaqMan assay for detection of canine parvovirus 2/feline panleukopenia virus (28) and to a minor groove binder probe assay for rapid discrimination between true feline panleukopenia virus strains and antigenic variants of canine parvovirus 2 (29). We also used DNA extracts to detect proviral DNA of feline immunodeficiency virus (30) and feline leukemia virus (31) and DNA of feline hemoplasmas (32) and feline herpesvirus (33). We screened RNA extracts by real-time PCR or conventional reverse transcription PCR specific for carnivore coronaviruses (34) and caliciviruses (33,35).

Results

Histopathologic Analysis

Figure 2

Thumbnail of Analysis of an orthopoxvirus isolated from an infected cat, Italy. A) Cytoplasmic fluorescence in infected Vero cells using serum from the diseased cat (original magnification ×400). B) Cytoplasmic inclusion bodies (arrows) in infected Vero cells (hematoxylin and eosin stain, original magnification ×400). C) Pocks (arrows) in the inoculated chorioallantoic membrane of a 12-day-old chick embryo. D) Electron micrograph of orthopoxvirus-like particle from infected Vero cells. The virus

Figure 2. Analysis of an orthopoxvirus isolated from an infected cat, Italy. A) Cytoplasmic fluorescence in infected Vero cells using serum from the diseased cat (original magnification ×400). B) Cytoplasmic inclusion bodies (arrows)...

Histopathologic analysis of multiple skin specimens showed mild hyperplasia of the epidermis and the follicular wall. Many roundish to oval brightly eosinophilic inclusion bodies were clearly evident in the cytoplasm of both epidermal and follicular keratinocytes, including in a few sebocytes. The morphology of cells suggested a possible OPXV infection (Figure 2, panel A). Nodular to diffuse dermatitis caused by mixed inflammatory cells was also present in dermis and hypodermis; those cells were mainly represented by eosinophils, histiocytes, and lymphocytes, together with few plasma cells and neutrophils.

Molecular Investigations

Molecular analysis of formalin-fixed, paraffin-embedded tissues showed positive results for the low GC panchordopoxvirus PCR and negative results for the high GC panchordopoxvirus PCR (19). This pattern of amplification was consistent with an OPXV infection. Amplification of the gene coding for the A-type inclusion protein generated an amplicon of ≈1,237 bp, and amplification of the HA gene (20,21) generated an amplicon of 846 bp, which are expected sizes for these genes in ECTV. All samples collected from the cat were negative for other pathogens by the molecular assays used.

Sequence analysis of the HA gene of strain Italy_09/17 showed high nucleotide identity (98%) with that of CPXV strain Germany (GenBank accession no. HQ420897) and to feline-derived human poxvirus IT1 (accession no. EF612709). In addition, strain Italy_09/17 was also highly related to most of the ECTV strains in GenBank; the highest (97%) nucleotide identity was with ECTV strain Naval (accession no. KJ563295). Strain Italy_09/17 showed positive results in the ECTV-specific PCR and negative results in the CPXV-specific PCR (22) (Table 1).

Virus Isolation

Virus isolation from freshly collected skin biopsy specimens was successful with Vero and CV-1 cells. We observed a cytopathic effect at 48 hours postinfection that showed rounding of cells, increased granularity, and detachment from the monolayer. In Vero cells, a cytopathic effect was less evident than in CV-1 cells. Cells stained with hematoxylin and eosin contained large eosinophilic cytoplasmic inclusion bodies that were compatible with infection by poxviruses, including CPXV (36) and ECTV (37) (Figure 2, panel B).

The IIF assay showed granular fluorescence areas that displayed the morphology of the inclusion bodies in cell cytoplasms (Figure 2, panel C). Both CV-1 and Vero cells showed positive IIF assay results, but there was no fluorescence staining in the negative control.

At 48 hours postinoculation on embryonated eggs, virus produced superficial pocks on the chorioallantoic membrane. Most of these pocks were small (diameter 1.0 mm), gray, and had central hemorrhages. Few (3%–5%) pocks were larger (1.8 mm in diameter), white, and without hemorrhages.

Electron Microscopy

Many typical brick-shaped virions (≈320 × 240 nm) morphologically related to the genus Orthopoxvirus were observed by negative staining and electron microscopy. We observed these results for skin punch biopsy specimens and cell culture supernatants.

As in a previous study (15), few particles showed the characteristic ribbon structure of the M form of vaccinia virus (38) (Figure 2, panel D), which is usually prevalent in fresh preparations collected during acute-phase infections. Most virions were slightly larger, showed a uniform electron density, and had a thick capsule outlined by a ragged edge (i.e., the morphologic aspect known as the C form), which are less infective and prevalent during evolution of a chronic infection.

Serologic Analysis

The infected cat was negative by virus neutralization for strain Italy_09/17 and reference VACV isolates. However, the IIF assay detected antibody titers of 1:1,280 for virus Italy_09/17 and 1:640 for VACV-WR.

Identification of a Novel OPXV by NGS

We used 217,236 paired reads for de novo assembling and obtained 3 contigs (contig one, 195,015 bp; contig two, 21,014 bp; and contig three, 1,596 bp) and a quality score >99%. The mean coverage of the assembled contigs was 61×. The 9 open reading frames (A7L, A10L, A24R, D1R, D5R, E6R, E9L, H4L, and J6R) used for OPXV characterization were mapped in contig 1, and their sequences (total 27,228 nt) were concatenated and aligned with concatenated cognate sequences of selected OPXVs. In addition, because the HA gene of 2 feline-derived human virus isolates was available in the sequence databases, we performed an alignment based on the HA gene. We conducted phylogenetic analysis on the basis of the 9 concatenated sequences by using Bayesian inference. Posterior probabilities percentages were consistently high (>90%) for all clades on phylograms, which supported inferred phylogenetic relationships.

Figure 3

Thumbnail of Phylogenetic relationship of extant orthopoxviruses with a feline poxvirus isolated from a cat, Italy. Phylogenetic tree shows 27,228 nt concatenated alignment of 9 coding gene (A7L, A10L, A24R, D1R, D5R, E6R, E9L, H4L, and J6R) sequences of orthopoxvirus. Gene designations refer to the VACV-COP genome (GenBank accession no. M35027). Posterior output of the tree was derived from Bayesian inference using 4 chains run for >1 million generations, a general time reversible model, a p

Figure 3. Phylogenetic relationship of extant orthopoxviruses with a feline poxvirus isolated from a cat, Italy. Phylogenetic tree shows 27,228 nt concatenated alignment of 9 coding gene (A7L, A10L, A24R, D1R, D5R, E6R,...

In the consensus phylogenetic tree (Figure 3), we found that strain Italy_09/17 was distantly related to other OPXVs, including all 10 CPXV lineages (39) and other recently identified, deep-branching OPXVs (40,41) and displayed a closer relatedness with ECTV prototypes, albeit forming a separate cluster. This cluster also included strain Abatino, which was recently isolated from a poxvirus outbreak in a captive colony of Tonkean macaques in Italy (42). Nucleotide identity of strain Italy_09/17 with strain Abatino was 99.66% and identity with reference ECTVs was 98.11%–98.13%. Higher nucleotide identities were found among ECTVs (99.97%–99.99%) and between VARV-Garcia1966 (variola minor) and VARV-India1967 (variola major) (99.68%). Thus, on the basis of current OPXV criteria of species demarcation, the cat and macaque isolates should be considered prototypes of a novel OPXV. Also, for the HA gene, strain Italy_09/17 appeared more closely related to strain Abatino (99.79% nt identity) than to feline-derived human OPXV strains (95.83%–95.99% nt identity) that were identified in Italy in 2009, for which a full-length genome and concatenated genes used for species demarcation using phylogeny are not available (43).

Discussion

OPXV infection in cats is frequently observed, and OPXV transmission from cats to humans has been demonstrated or at least suspected on several occasions (8,11,14,43–47). Cats are susceptible to CPXV infection, for which they represent only incidental hosts, as are humans, cattle, horses, and dogs. The virus is usually transmitted to cats by hunted rodents; cat-to-cat transmission is apparently rare (47). In contrast, ECTV has a host range restricted to laboratory mice, and cat or human infections have not been reported (6).

Additional OPXVs, such as raccoonpox virus and skunkpox virus, have been reported in wildlife and infect carnivores (48). Conversely, cats have been found to be susceptible to members of the genus Parapoxvirus, raccoonpox virus, and uncharacterized poxviruses (49). There are >400 reports of OPXV infection in domestic cats, but the total number of feline cases is considered to be much greater (5). Despite this large number of reports, genetic characterization of the detected poxvirus has been achieved in only a few instances. Thus, circulation in cats of other OPXVs cannot be ruled out.

We report detection of an OPXV strain that caused a fatal infection in a cat. The virus was not a classical CPXV, which is common in felids. Analysis of 9 concatenated genes showed that the poxvirus detected was only distantly related to all CPXV lineages currently known and formed a separate cluster with respect to ECTV, with which it was strictly related and grouped with an OPXV strain recently isolated from captive macaques in Italy (42). These 2 viruses had lower genetic identity with ECTV than that observed with reference ECTVs and between variola minor virus and variola major virus. Therefore, these ECTV-like poxviruses likely represent a novel OPXV species. However, the true animal reservoir of this novel OPXV needs to be assessed, and the idea that wild rodents can act as carriers for the new virus cannot be ruled out.

If one considers the close relatedness between strain Italy_09/17 and ECTV, which has been detected only in laboratory animals, it could be speculated that an ECTV-like virus circulating in wild rodents has resulted in ECTV strains adapted to laboratory mice. Alternatively, an ECTV strain might have escaped from laboratory mice and adapted to wild conditions. In addition, the zoonotic potential of the feline ECTV-like OPXV deserves an in-depth investigation. Feline poxvirus was also related to an unclassified OPXV, which was detected in a human in Italy almost 10 years ago and for which only partial HA gene has been identified (43). Consequently, this feline poxvirus could represent a threat to human health. Thus, veterinarians and cat breeders and owners should be aware of this additional risk associated with handling of cats with skin lesions.

Dr. Lanave is a postdoctoral fellow in the Department of Veterinary Medicine, University of Bari, Bari, Italy. His primary research interest is emerging viruses of animals.

Top

Acknowledgments

We thank Costantina Desario and Carlo Armenise for providing excellent technical assistance and G. Tekes for providing the VACV-WR strain and CV-1 cells.

This study was supported by grants from the University of Bari.

Top

References

  1. Centers for Disease Control and Prevention. Bioterrorism agents/diseases, 2015 [cited 2015 Nov 18] http://www.bt.cdc.gov/agent/agentlist-category.asp
  2. Reynolds  MG, Carroll  DS, Karem  KL. Factors affecting the likelihood of monkeypox’s emergence and spread in the post-smallpox era. Curr Opin Virol. 2012;2:335–43. DOIPubMedGoogle Scholar
  3. Hendrickson  RC, Wang  C, Hatcher  EL, Lefkowitz  EJ. Orthopoxvirus genome evolution: the role of gene loss. Viruses. 2010;2:1933–67. DOIPubMedGoogle Scholar
  4. Kinnunen  PM, Henttonen  H, Hoffmann  B, Kallio  ER, Korthase  C, Laakkonen  J, et al. Orthopox virus infections in Eurasian wild rodents. Vector Borne Zoonotic Dis. 2011;11:1133–40. DOIPubMedGoogle Scholar
  5. Essbauer  S, Pfeffer  M, Meyer  H. Zoonotic poxviruses. Vet Microbiol. 2010;140:229–36. DOIPubMedGoogle Scholar
  6. Esteban  DJ, Buller  RM. Ectromelia virus: the causative agent of mousepox. J Gen Virol. 2005;86:2645–59. DOIPubMedGoogle Scholar
  7. Osterhaus  AD, Teppema  JS, Wirahadiredja  RM, van Steenis  G. Mousepox in the Netherlands. Lab Anim Sci. 1981;31:704–6.PubMedGoogle Scholar
  8. Vorou  RM, Papavassiliou  VG, Pierroutsakos  IN. Cowpox virus infection: an emerging health threat. Curr Opin Infect Dis. 2008;21:153–6. DOIPubMedGoogle Scholar
  9. Schaudien  D, Meyer  H, Grunwald  D, Janssen  H, Wohlsein  P. Concurrent infection of a cat with cowpox virus and feline parvovirus. J Comp Pathol. 2007;137:151–4. DOIPubMedGoogle Scholar
  10. Schöniger  S, Chan  DL, Hollinshead  M, Humm  K, Smith  GL, Beard  PM. Cowpox virus pneumonia in a domestic cat in Great Britain. Vet Rec. 2007;160:522–3. DOIPubMedGoogle Scholar
  11. Schulze  C, Alex  M, Schirrmeier  H, Hlinak  A, Engelhardt  A, Koschinski  B, et al. Generalized fatal Cowpox virus infection in a cat with transmission to a human contact case. Zoonoses Public Health. 2007;54:31–7. DOIPubMedGoogle Scholar
  12. Johnson  MS, Martin  M, Stone  B, Hetzel  U, Kipar  A. Survival of a cat with pneumonia due to cowpox virus and feline herpesvirus infection. J Small Anim Pract. 2009;50:498–502. DOIPubMedGoogle Scholar
  13. Kaysser  P, von Bomhard  W, Dobrzykowski  L, Meyer  H. Genetic diversity of feline cowpox virus, Germany 2000-2008. Vet Microbiol. 2010;141:282–8. DOIPubMedGoogle Scholar
  14. Herder  V, Wohlsein  P, Grunwald  D, Janssen  H, Meyer  H, Kaysser  P, et al. Poxvirus infection in a cat with presumptive human transmission. Vet Dermatol. 2011;22:220–4. DOIPubMedGoogle Scholar
  15. Canese  MG, Lavazza  A, Massone  A, Galeano  F, Boldini  M. Feline poxvirus infection. A case report. Schweiz Arch Tierheilkd. 1997;139:454–7.PubMedGoogle Scholar
  16. Haenssle  HA, Kiessling  J, Kempf  VA, Fuchs  T, Neumann  C, Emmert  S. Orthopoxvirus infection transmitted by a domestic cat. J Am Acad Dermatol. 2006;54(Suppl):S1–4. DOIPubMedGoogle Scholar
  17. Schiavi  S, Vercelli  A, Abtamo  FU. A case of viral poxvirus dermatitis in a cat [in Italian]. Presented at the Congress of the Italian Society of Veterinary Dermatology; March 11, 2007; Cremona, Italy.
  18. Appl  C, von Bomhard  W, Hanczaruk  M, Meyer  H, Bettenay  S, Mueller  R. Feline cowpoxvirus infections in Germany: clinical and epidemiological aspects. Berl Munch Tierarztl Wochenschr. 2013;126:55–61.PubMedGoogle Scholar
  19. Li  Y, Meyer  H, Zhao  H, Damon  IK. GC content-based pan-pox universal PCR assays for poxvirus detection. J Clin Microbiol. 2010;48:268–76. DOIPubMedGoogle Scholar
  20. Meyer  H, Ropp  SL, Esposito  JJ. Gene for A-type inclusion body protein is useful for a polymerase chain reaction assay to differentiate orthopoxviruses. J Virol Methods. 1997;64:217–21. DOIPubMedGoogle Scholar
  21. Ropp  SL, Jin  Q, Knight  JC, Massung  RF, Esposito  JJ. Polymerase chain reaction strategy for identification and differentiation of smallpox and other orthopoxviruses. J Clin Microbiol. 1995;33:2069–76.PubMedGoogle Scholar
  22. Meyer  H, Damon  IK, Esposito  JJ. Orthopoxvirus diagnostics. Methods Mol Biol. 2004;269:119–34.PubMedGoogle Scholar
  23. Andrews  S. FastQC: a quality control tool for high throughput sequence data, 2010 [cited 2018 May 15]. http://www.bioinformatics.bbsrc.ac.uk/projects/fastqc/
  24. Emerson  GL, Li  Y, Frace  MA, Olsen-Rasmussen  MA, Khristova  ML, Govil  D, et al. The phylogenetics and ecology of the orthopoxviruses endemic to North America. PLoS One. 2009;4:e7666. DOIPubMedGoogle Scholar
  25. Katoh  K, Misawa  K, Kuma  K, Miyata  T. MAFFT: a novel method for rapid multiple sequence alignment based on fast Fourier transform. Nucleic Acids Res. 2002;30:3059–66. DOIPubMedGoogle Scholar
  26. Huelsenbeck  JP, Ronquist  F. MRBAYES: Bayesian inference of phylogenetic trees. Bioinformatics. 2001;17:754–5. DOIPubMedGoogle Scholar
  27. Ronquist  F, Huelsenbeck  JP. MrBayes 3: Bayesian phylogenetic inference under mixed models. Bioinformatics. 2003;19:1572–4. DOIPubMedGoogle Scholar
  28. Decaro  N, Elia  G, Martella  V, Desario  C, Campolo  M, Trani  LD, et al. A real-time PCR assay for rapid detection and quantitation of canine parvovirus type 2 in the feces of dogs. Vet Microbiol. 2005;105:19–28. DOIPubMedGoogle Scholar
  29. Decaro  N, Desario  C, Lucente  MS, Amorisco  F, Campolo  M, Elia  G, et al. Specific identification of feline panleukopenia virus and its rapid differentiation from canine parvoviruses using minor groove binder probes. J Virol Methods. 2008;147:67–71. DOIPubMedGoogle Scholar
  30. Stiles  J, Bienzle  D, Render  JA, Buyukmihci  NC, Johnson  EC. Use of nested polymerase chain reaction (PCR) for detection of retroviruses from formalin-fixed, paraffin-embedded uveal melanomas in cats. Vet Ophthalmol. 1999;2:113–6. DOIPubMedGoogle Scholar
  31. Quackenbush  SL, Dean  GA, Mullins  JI, Hoover  EA. Analysis of FeLV-FAIDS provirus burden and productive infection in lymphocyte subsets in vivo. Virology. 1996;223:1–9. DOIPubMedGoogle Scholar
  32. Tasker  S, Binns  SH, Day  MJ, Gruffydd-Jones  TJ, Harbour  DA, Helps  CR, et al. Use of a PCR assay to assess the prevalence and risk factors for Mycoplasma haemofelis and ‘Candidatus Mycoplasma haemominutum’ in cats in the United Kingdom. Vet Rec. 2003;152:193–8. DOIPubMedGoogle Scholar
  33. Di Martino  B, Di Francesco  CE, Meridiani  I, Marsilio  F. Etiological investigation of multiple respiratory infections in cats. New Microbiol. 2007;30:455–61.PubMedGoogle Scholar
  34. Gut  M, Leutenegger  CM, Huder  JB, Pedersen  NC, Lutz  H. One-tube fluorogenic reverse transcription-polymerase chain reaction for the quantitation of feline coronaviruses. J Virol Methods. 1999;77:37–46. DOIPubMedGoogle Scholar
  35. Jiang  X, Huang  PW, Zhong  WM, Farkas  T, Cubitt  DW, Matson  DO. Design and evaluation of a primer pair that detects both Norwalk- and Sapporo-like caliciviruses by RT-PCR. J Virol Methods. 1999;83:145–54. DOIPubMedGoogle Scholar
  36. Downie  AW. A study of the lesions produced experimentally by cowpox virus. J Pathol Bacteriol. 1939;48:361–79. DOIGoogle Scholar
  37. Barnard  JE, Elford  WJ. The causative organism in infectious ectromelia. Proceedings of the Royal Society, Series B. 1931;109:360–80. DOIGoogle Scholar
  38. Westwood  JC, Harris  WJ, Zwartouw  HT, Titmuss  DH, Appleyard  G. Studies on the structure of vaccinia virus. J Gen Microbiol. 1964;34:67–78. DOIPubMedGoogle Scholar
  39. Mauldin  MR, Antwerpen  M, Emerson  GL, Li  Y, Zoeller  G, Carroll  DS, et al. Cowpox virus: What’s in a Name? Viruses. 2017;9:E101. DOIPubMedGoogle Scholar
  40. Springer  YP, Hsu  CH, Werle  ZR, Olson  LE, Cooper  MP, Castrodale  LJ, et al. Novel orthopoxvirus infection in an Alaska resident. Clin Infect Dis. 2017;64:1737–41. DOIPubMedGoogle Scholar
  41. Vora  NM, Li  Y, Geleishvili  M, Emerson  GL, Khmaladze  E, Maghlakelidze  G, et al. Human infection with a zoonotic orthopoxvirus in the country of Georgia. N Engl J Med. 2015;372:1223–30. DOIPubMedGoogle Scholar
  42. Cardeti  G, Gruber  CEM, Eleni  C, Carletti  F, Castilletti  C, Manna  G, et al. Fatal outbreak in Tonkean macaques caused by possibly novel orthopoxvirus, Italy, January 2015. Emerg Infect Dis. 2017;23:1941–9. DOIPubMedGoogle Scholar
  43. Carletti  F, Bordi  L, Castilletti  C, Di Caro  A, Falasca  L, Gioia  C, et al. Cat-to-human orthopoxvirus transmission, northeastern Italy. Emerg Infect Dis. 2009;15:499–500. DOIPubMedGoogle Scholar
  44. Eis-Hübinger  AM, Gerritzen  A, Schneweis  KE, Pfeiff  B, Pullmann  H, Mayr  A, et al. Fatal cowpox-like virus infection transmitted by cat. Lancet. 1990;336:880. DOIPubMedGoogle Scholar
  45. Schupp  P, Pfeffer  M, Meyer  H, Burck  G, Kölmel  K, Neumann  C. Cowpox virus in a 12-year-old boy: rapid identification by an orthopoxvirus-specific polymerase chain reaction. Br J Dermatol. 2001;145:146–50. DOIPubMedGoogle Scholar
  46. Hawranek  T, Tritscher  M, Muss  WH, Jecel  J, Nowotny  N, Kolodziejek  J, et al. Feline orthopoxvirus infection transmitted from cat to human. J Am Acad Dermatol. 2003;49:513–8. DOIPubMedGoogle Scholar
  47. Świtaj  K, Kajfasz  P, Kurth  A, Nitsche  A. Cowpox after a cat scratch - case report from Poland. Ann Agric Environ Med. 2015;22:456–8. DOIPubMedGoogle Scholar
  48. International Committee on Taxonomy of Viruses. Virus taxonomy: 2016 release, 2017 [cited 2018 May 15]. https://talk.ictvonline.org/taxonomy/
  49. Greene  CE. Poxvirus infections. In: Greene CE, editor. Infectious diseases of the dog and cat. 4th ed. St. Louis: Saunders Elsevier; 2006. p. 166–9.

Top

Figures
Tables

Top

Cite This Article

DOI: 10.3201/eid2409.171283

Original Publication Date: July 23, 2018

Table of Contents – Volume 24, Number 9—September 2018

EID Search Options
presentation_01 Advanced Article Search – Search articles by author and/or keyword.
presentation_01 Articles by Country Search – Search articles by the topic country.
presentation_01 Article Type Search – Search articles by article type and issue.

Top

Comments

Please use the form below to submit correspondence to the authors or contact them at the following address:

Nicola Decaro, Department of Veterinary Medicine, University of Bari, Strada Provinciale per Casamassima Km 3, 70010 Valenzano, Bari, Italy

Send To

10000 character(s) remaining.

Top

Page created: August 14, 2018
Page updated: August 14, 2018
Page reviewed: August 14, 2018
The conclusions, findings, and opinions expressed by authors contributing to this journal do not necessarily reflect the official position of the U.S. Department of Health and Human Services, the Public Health Service, the Centers for Disease Control and Prevention, or the authors' affiliated institutions. Use of trade names is for identification only and does not imply endorsement by any of the groups named above.
file_external