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Volume 26, Number 8—August 2020

Virome Analysis for Detection of Segmented Flaviviruses in Wild Rodents, Pennsylvania, USA

Arvind Kumar1, Kurt J. Vandegrift1, Himanshu Sharma, Satyapramod Murthy, Laura D. Kramer, Richard Ostfeld, Peter Hudson, and Amit KapoorComments to Author 
Author affiliations: Center for Vaccines and Immunity, The Abigail Wexner Research Institute at Nationwide Children’s Hospital, Columbus, Ohio, USA (A. Kumar, H. Sharma, S. Murthy, A. Kapoor); Center for Infectious Disease Dynamics, Pennsylvania State University, University Park, Pennsylvania, USA (K.J. Vandegrift, P. Hudson); Wadsworth Center, New York State Department of Health, Albany, New York, USA (L.D. Kramer); University of Albany-SUNY School of Public Health, Albany (L.D. Kramer)

Suggested citation for this article


Identifying viruses in synanthropic animals is necessary for understanding the origin of many viruses that can infect human hosts and developing strategies to prevent new zoonotic infections. The white-footed mouse, Peromyscus leucopus, is one of the most abundant rodent species in the northeastern United States. We characterized the serum virome of 978 free-ranging P. leucopus mice caught in Pennsylvania. We identified many new viruses from 26 different virus families. Among these viruses was a highly divergent segmented flavivirus whose genetic relatives were recently identified in ticks, mosquitos, and vertebrates, including febrile patients. The novel flavi-like segmented virus, isolated from ticks in Pennsylvania, shares ˂70% aa identity with known viruses in the highly conserved region of the viral polymerase. Our data will enable researchers to develop molecular reagents to further characterize this virus and its relatives infecting other hosts and to curtail their spread, if necessary.

Most human infectious diseases have a zoonotic origin (1). RNA viruses are remarkable in their ability to evolve and infect a wide range of hosts, primarily due to their error-prone replication, small genome size, and ability to adapt (2). Recent studies describing human infections from animal coronaviruses and paramyxoviruses illustrate well the high zoonotic potential of animal RNA viruses (3). Not all viruses at the human–animal interface can breach the species barrier, and successful cross-species transmission often requires repeated introduction coupled with favorable circumstances (3). These multiple exposures also provide increased opportunity for viral adaptation, and because humans are frequently exposed to viruses from synanthropic hosts, this channel becomes a clear route of infection. As such, we need to identify and characterize viruses from synanthropic animals to understand the origins of many human viruses and obtain insights into the emergence of potential zoonotic infections (1).

Rodents and bats represent a common source of potential zoonotic viruses (4). In the northeastern United States, the white-footed mouse (Peromyscus leucopus) is one of the most widespread and abundant rodent species. These mice are highly adaptable, commonly become synanthropic, and invade human domiciles in the fall. It is plausible that humans are exposed to a wide range of viruses from these mice, either directly as in the case with hantaviruses or indirectly through vectors such as ticks. Indeed, these mice are known to harbor a range of zoonotic pathogens, including the tickborne Borrelia burgdorferi, which causes Lyme disease, and Anaplasma phagocytilium, which causes anaplasmosis (5). White-footed mice can also act as reservoirs for bacteria that are causative agents of Rocky Mountain spotted fever, tularemia, plague, and bartonellosis and for protozoans responsible for babesiosis, giardiasis, toxoplasmosis, and cryptosporidiosis (6). Infectious viruses reported in P. leucopus include lymphocytic choriomeningitis virus, Powassan or deer tick encephalitis virus, and hantaviruses (7,8).

The genome of flaviviruses is composed of a single-stranded positive-sense RNA that codes for a single polyprotein. The genome of Jingmen tick virus (JMTV), which was first identified in 2014 from ticks in the Jingmen province of China (9), is composed of 4 single-stranded positive-sense RNA segments, 2 of which encode a polymerase protein (NS5) and a helicase protein (NS3) that show close phylogenetic relatedness with the corresponding proteins of classical flaviviruses (9). Later, several genetically diverse relatives of JMTV were found in several species of ticks, insects, and mammals (913). Together, these JMTV-like viruses are highly diverse and show differences in the number of genomic segments as well as protein coding strategies (9,10,12). In 2018, a metagenomics study revealed the presence of JMTV-like sequences in serum samples from human patients with Crimean-Congo hemorrhagic fever in Kosovo (14). Two studies published in 2019 reported the presence of JMTV sequences in patients in China with febrile illness and a history of recent tick bites (15,16). To date, no information is available on the presence of JMTV infections in insects, ticks, or vertebrates in North America.

Knowledge about viruses infecting P. leucopus and the levels to which humans are being exposed is limited. Whereas several studies have examined the prevalence of hantaviruses (17) and highly diverse hepaciviruses (18), there has been no attempt to characterize the blood virome of these common rodents. We used an unbiased, metaviromics approach to identify all viruses in the serum samples of 978 free-ranging white-footed mice captured over a period of 7 years from suburban and wild areas of Pennsylvania.

Materials and Methods

Origin and Details of White-Footed Mouse Samples

We collected serum samples from P. leucopus mice each spring and autumn during 2011–2017 from 4 sites in central Pennsylvania. We selected these sites because they provided gradient levels of human activity and so exposure to rodents; site 1 had the highest level of exposure and site 4 had the lowest. At site 1 (Deer Pens), mouse infestation is reported in residences, workplaces, and the surrounding area, providing a potentially high level of exposure to rodents. Site 2 (Spray Fields) is a disturbed forest where treated wastewater is sprayed; it is frequented daily by maintenance employees and dog walkers, but there are no residences on site. Site 3 (Scotia) is on Pennsylvania state game land that borders housing communities and has mostly seasonal visitors, such as hikers, hunters, and trappers. Site 4 (Stone Valley) is in a large contiguous forest that has very few people or residences. Additional details about the sites have been described previously (19).

Whole blood was obtained from the retro-orbital sinus of the anesthetized mice. These blood samples were centrifuged at 8,000 × g for 10 min and the serum then collected with a micropipette. Samples were stored at −80°C. All procedures were approved by Penn State’s Institutional Animal Care and Use Committee (IACUC #46246).

Metagenomics, Metaviromics, and Bioinformatics

We used serum samples from 978 wild free-ranging P. leucopus mice to generate the high-throughput sequence data to characterize the virome of these rodents. We used a 10-µL subsample of serum from each individual mouse to create 9 pools. We assigned individual mice to pools by bodyweight (as a proxy for age) and study site. We centrifuged serum pools at 8,000 × g for 10 min to remove particulate matter. The supernatants were treated with DNase (100 U), RNase (20 U), and Benzonase (250 U) to enrich samples for particle-protected (virion) nucleic acids. We used the QIAamp Viral RNA Mini Kit (QIAGEN Inc., to extract nucleic acid from the serum pools and eluted it in 60 μL of elution buffer supplemented with 40 units of ribonuclease inhibitor, then stored at it −80°C before processing it for library preparation. We used a unique 20-nt barcoded oligonucleotide primer for each sample pool during reverse transcription PCR (RT-PCR) and second-strand DNA synthesis, as previously described (20). We prepared libraries for Illumina sequencing as previously described (21) and performed sequencing on a HiSeq 4000 platform (Illumina Inc., for 2 × 150 cycles in the Biomedicine Genomics Core at the Research Institute of Nationwide Children’s Hospital (Columbus, Ohio, USA).

We used the 20-nt unique barcodes included in the primers used to make libraries to demultiplex sequence data. After removing low-complexity regions and low-quality bases, we aligned paired‐end reads to the P. leucopus genomes with Bowtie2 mapper version 2.0.6 (SourceForge, to remove the host-derived sequences. We used MIRA version 4.0 (SourceForge) (22) for de novo assembly of remaining sequences. Finally, we analyzed all contigs and unique reads using MegaBLAST against the GenBank nonredundant nucleotide database. Next, we used BLASTX to analyze sequences that showed poor or no homology (e-score >0.001) against the viral GenBank protein database, followed by BLASTX against the nonredundant protein database. We then used reference genomes of known viruses available in GenBank to extract related sequences present in the 9 serum pools. Finally, we used specific PCR assays and traditional dideoxy sequencing of amplicons to confirm bioinformatics-based assembly of virus reads.

Presence and Prevalence of JMTV-Like and South Bay Viruses

We selected 2 viruses recently identified in ticks for further study: a highly divergent JMTV-like virus provisionally named flavi-like segmented virus–Pennsylvania (FLSV-PN), and South Bay virus (SBV), a newly identified tickborne virus that belongs to the family Nairoviridae, order Bunyavirales (23,24). We extracted individual serum samples included in the pool from 72 P. leucopus mice with the maximum number of unique FLSV-PN sequence reads and screened for the presence of FLSV-PN RNA using a nested RT-PCR targeting the conserved NS5 polymerase region. We used the primers FLSV-PN-F1 (5′-GGWGCYATGGGYTACCAGAT-3′) and FLSV-PN-R1 (5′-TCCARGGTGAGTARTCCTTTCG-3′) in the first round of PCR, and FLSV-PN-F2 (5′-GGWGCYATGGGYTACCAGATGGA-3′) and FLSV-PN-R2 (5′-CCARGGTGAGTARTCCTTTCGARATC-3′) in the second round. The first-round PCR cycle included 8 min of initial denaturation at 95°C; 10 cycles of 95°C for 40 s, 56°C for 1 min, and 72°C for 1 min; 30 cycles of 95°C for 30 s, 54°C for 30 s, and 72°C for 1 min; and a final extension at 72°C for 5 min. In the first 10 cycles, the annealing temperature was ramped down by 0.5°C each cycle to enable nucleotide mismatch tolerance during primer hybridization. The second-round PCR conditions included 8 min of initial denaturation at 95°C; 10 cycles of 95°C for 40 s, 60°C for 1 min, and 72°C for 1 min; 30 cycles of 95°C for 30 s, 58°C for 30 s, and 72°C for 1 min; and a final extension at 72°C for 5 min.

We used a heminested RT-PCR targeting the viral polymerase gene to screen serum samples from the same 72 mice for the presence of SBV. We used the primers SBV-F1 (5′-AYCCAGATTGGAARCACTTCATAATG-3′) and SBV-R1 (5′-CCATATGTDGTAATMACYTTWGCATA-3′) for first round of PCR, and SBV-F2 (5′-GTTATGTTGAAGGACCTTAACAAAG-3′) and SBV-R1 for the second round. The PCR cycle for both rounds of PCR included 8 min of initial denaturation at 95°C; 10 cycles of 95°C for 30 s, 55°C for 2 min, and 72°C for 1 min; 30 cycles of 95°C for 25 s, 54°C for 30 s, and 72°C for 30 s; and a final extension at 72°C for 5 min. In the first 10 cycles, the annealing temperature was ramped down by 0.5°C each cycle to enable nucleotide mismatch tolerance during primer hybridization step.

Phylogenetic Analysis and Genome Organization of FLSV-PN

We aligned sequences that showed substantial similarity with JMTV NS5 proteins with reference sequence YP_009029999.1 (GenBank accession no. MN811583) to design PCR primers for direct amplification of 2,568-nt FLSV-PN sequences. After we confirmed the FLSV-PN assembled sequence by Sanger sequencing, we aligned the translated protein sequence with the sequence of known JMTV-like viruses (aa 55 to 913 of NS5 protein) using BLOSUM protein weight matrix, using default parameters in MEGA 7.1 (25). We constructed a phylogenetic tree using the maximum-likelihood method and the best pattern substitution model with the lowest Bayesian information criterion score, LG+G+I model (Le Gascuel, Gamma distribution with 5 rate categories and evolutionary invariable sites) (26). To confirm that the FLSV-PN genome is segmented, we used FLSV-PN reads showing substantial similarity to JMTV NS3 protein for acquiring the 3′ end of FLSV-PN NS3 coding segment using a poly-T oligonucleotide-primed cDNA synthesis followed by specific PCR, as previously described (27). The 3′ end sequence of FLSV-PN NS3 coding segment and the complete 3′ untranslated region (UTR) is available in GenBank (accession no. MN811584).


Serum Virome of P. Leucopus

Figure 1

Thumbnail of Bubble plot showing the abundance of different viruses in the serum virome of the white-footed mouse. Sequence reads showing the highest sequence similarity to known viruses were normalized as reads per million and were grouped into RNA and DNA virus families. Read numbers were transformed to log2, where the cutoff is ≥2 reads, represented by the smallest circle.

Figure 1. Bubble plot showing the abundance of different viruses in the serum virome of the white-footed mouse. Sequence reads showing the highest sequence similarity to known viruses were normalized as reads per...

A total of 242 million paired-end sequences were generated from the 9 pools representing the serum samples of 978 P. leucopus. Of these, 148 million (61%) were derived from the host genome. Of the remaining 94 million sequences, 65.6% of reads showed substantial similarity to known viruses (e-value <0.001). Further analysis classified these sequences into 26 known RNA and DNA virus families (Figure 1).

DNA Virome

We found parvoviruses, circoviruses, Torque teno viruses (TTV), polyomaviruses, and papillomaviruses in all 9 serum pools, and these were the most abundant DNA viruses. Among parvoviruses, bocaparvoviruses (BocPV) sequences shared up to 90% aa identity with the nonstructural protein of a rodent BocPV identified in Brazil (28), and adeno-associated viruses (AAV) shared up to 65% aa identity with the nonstructural protein of a caprine AAV (29). The identified TTV sequences were genetically equidistant from rodent TTV (GenBank accession no. AEF5869) and mosquito TTV (GenBank accession no. AEF58766) (30); the sequences shared up to 60% aa identity with these 2 species of the genus Omegatorquevirus (31). The polyomavirus sequences shared up to 79% aa identity with the large T antigen of a polyomavirus isolated from the Montane grass mouse (Akodon montensis) (32). These papillomavirus sequences belong to a tentatively identified new virus species within the genus Iotapapillomavirus that shares up to 79% aa identity with the papillomavirus found in P. maniculatus (GenBank accession no. NC_039039) (33).

RNA Virome

The most abundant RNA viruses present in the P. leucopus serum pools were the genetically diverged variants of hepaciviruses and pegiviruses (34). Phylogenetic analyses of these sequences indicated that the P. leucopus hepaciviruses form a distinct new genetic cluster (35). We found sequence reads of a novel hepevirus in 8 of 9 serum pools. Genetic analysis of these P. leucopus hepevirus sequences suggest it is a new member of the genus Orthohepevirus because it shares <75% aa identity with the capsid proteins of hepevirus isolated from the common kestrel, Falco tinnunculus (36), and from rodents (37). Astrovirus-like sequences found in 8 serum pools shared up to 64% aa identity in the capsid protein and up to 73% aa identity in the nonstructural protein with the known species of the genus Mamastrovirus. Three of the 9 serum pools had sequences that were genetically closest to bat astroviruses (38) but shared up to 61% aa identity in the nonstructural protein. Sequences sharing up to 97% aa identity with hantaviruses recently found in Peromyscus sp. were also present in 6 serum pools (39). Coronavirus-related sequences were found in 2 serum pools and shared 98% aa identity with the porcine hemagglutinating encephalomyelitis virus (GenBank accession no. ACH72649). Paramyxovirus sequences were present in 5 serum pools and shared up to 90% nt identity with paramyxoviruses isolated from 3 rodent species: Apodemus peninsulae (accession no. KY370098), Rattus norvegicus (accession no. KX940961), and R. andamanensis (accession no. JN689227).

Rotavirus sequences were present in all serum pools and shared up to 78% nt identity in the NS3 gene with bovine rotavirus (GenBank accession no. JX442794) and human rotavirus (accession no. AB748601); <74% nt identity in the VP2 gene with avian rotavirus (accession no. FJ169854), human rotavirus (accession no. KF035108), and canine rotavirus (accession no. LC326510); and <45% aa identity in the VP6 gene to that of human RV (accession no. AHK24897) and canine RV (accession no. ACH97443). Picornavirus sequences were detected in 7 serum pools; these sequences shared up to 65% aa identity with marmot cardiovirus (accession no. AVX29481), <48% aa identity with rodent enterovirus (accession no. YP_009508417), <67% aa identity with Rattus tanezumi hunnivirus (accession no. AWK02689), and <87% aa identity with rodent hepatovirus (accession no. ALL35326).


We found sequences in 8 of the 9 P. leucopus serum pools almost identical to sequences in SBV. Because it was unknown whether the host range of this tickborne virus includes P. leucopus, we used RT-PCR assays to screen serum samples from 72 individual mice; 5 of the 72 were found to contain SBV variants sharing 99%–100% nt identity with the SBV identified in Ixodes scapularis ticks (24,40).

FLSV-PN We found 370 sequence reads that showed the highest sequence similarity with the NS5 proteins of JMTV-like viruses. Similarly, we found 42 sequence reads that showed the highest sequence similarity with the NS3 proteins of JMTV-like viruses (9,11,12,15). These FLSV-PN sequences were genetically equidistant from the 3 prototypic virus members of the JMTV-like virus group, namely JMTV, Mogiana tick virus, and Alongshan virus (15,16,24). Considering the potential consequentiality of a divergent JMTV-like virus infection in a widely distributed rodent species in North America, we developed a broadly reactive PCR assay to confirm our results and to define infection prevalence of FLSV-PN in P. leucopus mouse.

Figure 2

Thumbnail of Phylogenetic analyses of FLSV-PN (red) on the basis of NS5 proteins corresponding to amino acid positions 55 to 913 on Jingmen tick virus reference sequence YP_009029999.1. The trees are drawn to scale, with branch lengths measured in the number of substitutions per site.
A. Phylogenetic analysis of conventional flaviviruses (blue) and recently identified segmented flavi-like viruses from ticks, mosquitoes, and other arthropods. 
B. Phylogenetic analysis of viruses closely related t

Figure 2. Phylogenetic analyses of FLSV-PN (red) on the basis of NS5 proteins corresponding to amino acid positions 55 to 913 on Jingmen tick virus reference sequence YP_009029999.1. The trees are drawn to...

PCR screening and amplicon sequencing confirmed the presence of FLSV-PN nucleic acids in serum samples from 8 of the 72 mice in this pool, indicating an infection prevalence of 11%. Comparative sequence analysis determined ≈3.8% nt divergence in the NS5 region among FLSV-PN variants infecting these mice (data not shown); all of these mutations were synonymous. Next, we acquired the near-complete coding region for a FLSV-PN NS5 polymerase segment and used it for phylogenetic analysis (Figure 2). We determined that FLSV-PN is more genetically diverse than the previously identified JMTV variants and Alongshan virus and shared ˂70% aa identity with these viruses (Table). We used a poly-T oligonucleotide primed cDNA synthesis to acquire the 3′ end of FLSV-PN NS3 coding segment. Sequencing of the amplicon revealed the presence of a 388-nt 3′ untranslated region preceded by 96-aa NS3 protein coding region that showed distant yet highest significant sequence similarity with the carboxy terminal of JMTV NS3 protein. These results confirm that the FLSV-PN genome is segmented in the same way as JMTV-like viruses and that the FLSV-PN NS3 protein coding segment is polyadenylated.


Synanthropic small mammals serve as reservoirs for many zoonotic infections (4146). Mice of the genus Peromyscus are highly adaptable and thrive in human-modified landscapes. In particular, P. leucopus and P. maniculatus are closely related and very abundant in North America, with P. leucopus most common in the eastern two thirds of the United States, plus Canada and northern Mexico, and P. maniculatus present in the central and western United States. These rodents have been recognized as reservoirs of highly pathogenic hantaviruses, but the diversity of viruses infecting them has remained largely unknown. A recent study (18) showed the presence of highly diverse hepaciviruses and pegiviruses in these rodents, and a study published in 2011 by Phan et al. identified several other viruses in fecal samples of 20 P. leucopus mouse (47). Our study expands the host range of the recently identified tickborne virus SBV and identifies a highly diverse virus, FLSV-PN, whose genetic relatives were recently shown to be pathogenic for humans (15,16).

Our results show rich genetic diversity among viruses infecting these rodents. We not only confirmed infections from hantaviruses and hepaciviruses and pegiviruses but also found viruses representing homologs of almost all known viruses present in human serum samples: anelloviruses, parvoviruses, polyomaviruses, papillomaviruses, and hepatitis E virus. We also found several viruses not commonly present in human or animal serum samples, such as coronaviruses, paramyxoviruses, astroviruses, enteroviruses, and rotaviruses. It is plausible that some mice, when captured, had transient viremia of these otherwise respiratory or gastroenteric infections. It would therefore be worthwhile to further investigate other sample and tissue types including feces, skin, urine, saliva, and organs to identify additional viral diversity. This may also aid in determining the tissue tropism of these viruses and provide clues to potential routes of transmission.

Recently, an abundance of novel viruses has been identified in ticks from the United States (24); the host range and public health relevance of most of these new tickborne viruses remains unknown (24). We found 1 of these newly identified and highly prevalent tickborne viruses, SBV, in P. leucopus serum samples. To the best of our knowledge, SBV has not been detected in a mammalian host; our study indicates that this new tickborne virus can infect mammals and indeed may have a wider host range than was previously known. Comparative sequence analyses indicated that the SBV variants detected in P. leucopus serum samples share 99%–100% nt identity with the SBV variants identified in ticks, indicating shared ancestry and, possibly, mode of transmission.

Several recent studies to characterize the viromes of ticks and mosquitoes in North America showed an absence of JMTV-like viruses (24,40,48). Thus, our results indicate common FLSV infection in a wild rodent that is also a common host of ticks and mosquitoes in North America and raises questions about the source of FLSV-PN infection in these mice. It is plausible that FLSV-PN transmits through an arthropod vector other than ticks or mosquitoes; some distantly related viruses were found in pools of other insects and arachnids (10). It is also plausible that, akin to its close genetic relatives, FLSV-PN or related viruses can infect a range of animals, including humans. Because FLSV-PN is genetically distinct from all known JMTV-like virus species, recording its sequence data will be useful in identifying FLSV-PN–related viruses circulating in North America.

Dr. Kumar is a postdoctoral fellow at the Center of Vaccine and Immunity, Nationwide Children’s Hospital, Columbus, Ohio. His primary research interests include emerging virus discovery using next-generation sequencing and serologic approaches.



In conclusion, we found evidence of FLSV infections in a widespread mammalian species in North America, which is important because distant genetic relatives of FLSV-PN have been shown to be transmitted by ticks and mosquitoes (9,13) and readily able to infect humans (15,16). Until recently, these unusual flaviviruses had only been found in ticks, mosquitoes, and animals from China, Kosovo, and Brazil (11,14,16). However, in a 2019 article, Wang et al. reported finding JMTV viremia in 86 of 374 humans with febrile illness, headache, and history of tick exposure (16). In addition, JMTV was shown to replicate in several cell lines of human and animal origin (15,16). Taken together, these studies indicate that JMTV and related tickborne or insectborne viruses have the potential to infect a wide range of mammals, including humans.

Funding was provided by the National Science Foundation’s (NSF) Ecology and Evolution of Infectious Diseases program (grant number 1619072). K.J.V. and part of the field work were supported by the Institutes for Energy and the Environment of Pennsylvania State University through a grant to PJH.



  1. Woolhouse  MEJ, Gowtage-Sequeria  S. Host range and emerging and reemerging pathogens. Emerg Infect Dis. 2005;11:18427. DOIPubMed
  2. Holmes  EC. The evolution and emergence of RNA viruses. Oxford: Oxford University Press; 2009.
  3. Plowright  RK, Parrish  CR, McCallum  H, Hudson  PJ, Ko  AI, Graham  AL, et al. Pathways to zoonotic spillover. Nat Rev Microbiol. 2017;15:50210. DOIPubMed
  4. Luis  AD, Hayman  DTS, O’Shea  TJ, Cryan  PM, Gilbert  AT, Pulliam  JRC, et al. A comparison of bats and rodents as reservoirs of zoonotic viruses: are bats special? Proc Biol Sci. 2013;280:20122753. DOIPubMed
  5. Hersh  MH, Ostfeld  RS, McHenry  DJ, Tibbetts  M, Brunner  JL, Killilea  ME, et al. Co-infection of blacklegged ticks with Babesia microti and Borrelia burgdorferi is higher than expected and acquired from small mammal hosts. PLoS One. 2014;9:e99348. DOIPubMed
  6. Barbour  AG. Infection resistance and tolerance in Peromyscus spp., natural reservoirs of microbes that are virulent for humans. Semin Cell Dev Biol. 2017;61:11522. DOIPubMed
  7. Gage  KL, Ostfeld  RS, Olson  JG. Nonviral vector-borne zoonoses associated with mammals in the United States. J Mammal. 1995;76:695715. DOI
  8. Childs  JE, Ksiazek  TG, Spiropoulou  CF, Krebs  JW, Morzunov  S, Maupin  GO, et al. Serologic and genetic identification of Peromyscus maniculatus as the primary rodent reservoir for a new hantavirus in the southwestern United States. J Infect Dis. 1994;169:127180. DOIPubMed
  9. Qin  XC, Shi  M, Tian  JH, Lin  XD, Gao  DY, He  JR, et al. A tick-borne segmented RNA virus contains genome segments derived from unsegmented viral ancestors. Proc Natl Acad Sci U S A. 2014;111:67449. DOIPubMed
  10. Shi  M, Lin  XD, Vasilakis  N, Tian  JH, Li  CX, Chen  LJ, et al. Divergent viruses discovered in arthropods and vertebrates revise the evolutionary history of the Flaviviridae and related viruses. J Virol. 2015;90:65969. DOIPubMed
  11. Villa  EC, Maruyama  SR, de Miranda-Santos  IKF, Palacios  G, Ladner  JT. Complete coding genome sequence for Mogiana tick virus, a Jingmenvirus isolated from ticks in Brazil. Genome Announc. 2017;5:e00232-17. DOIPubMed
  12. Ladner  JT, Wiley  MR, Beitzel  B, Auguste  AJ, Dupuis  AP II, Lindquist  ME, et al. A multicomponent animal virus isolated from mosquitoes. Cell Host Microbe. 2016;20:35767. DOIPubMed
  13. Souza  WM, Fumagalli  MJ, Torres Carrasco  AO, Romeiro  MF, Modha  S, Seki  MC, et al. Viral diversity of Rhipicephalus microplus parasitizing cattle in southern Brazil. Sci Rep. 2018;8:16315. DOIPubMed
  14. Emmerich  P, Jakupi  X, von Possel  R, Berisha  L, Halili  B, Günther  S, et al. Viral metagenomics, genetic and evolutionary characteristics of Crimean-Congo hemorrhagic fever orthonairovirus in humans, Kosovo. Infect Genet Evol. 2018;65:611. DOIPubMed
  15. Jia  N, Liu  HB, Ni  XB, Bell-Sakyi  L, Zheng  YC, Song  JL, et al. Emergence of human infection with Jingmen tick virus in China: A retrospective study. EBioMedicine. 2019;43:31724. DOIPubMed
  16. Wang  ZD, Wang  B, Wei  F, Han  SZ, Zhang  L, Yang  ZT, et al. A new segmented virus associated with human febrile illness in China. N Engl J Med. 2019;380:211625. DOIPubMed
  17. Song  JW, Baek  LJ, Nagle  JW, Schlitter  D, Yanagihara  R. Genetic and phylogenetic analyses of hantaviral sequences amplified from archival tissues of deer mice (Peromyscus maniculatus nubiterrae) captured in the eastern United States. Arch Virol. 1996;141:95967. DOIPubMed
  18. Kapoor  A, Simmonds  P, Scheel  TKH, Hjelle  B, Cullen  JM, Burbelo  PD, et al. Identification of rodent homologs of hepatitis C virus and pegiviruses. MBio. 2013;4:e0021613. DOIPubMed
  19. Vandegrift  KJ, Hudson  PJ. Could parasites destabilize mouse populations? The potential role of Pterygodermatites peromysci in the population dynamics of free-living mice, Peromyscus leucopus. Int J Parasitol. 2009;39:125362. DOIPubMed
  20. Moser  LA, Ramirez-Carvajal  L, Puri  V, Pauszek  SJ, Matthews  K, Dilley  KA, et al. A universal next-generation sequencing protocol to generate noninfectious barcoded cDNA libraries from high-containment RNA viruses. mSystems. 2016;1:e00039-15. DOIPubMed
  21. Kapoor  A, Kumar  A, Simmonds  P, Bhuva  N, Singh Chauhan  L, Lee  B, et al. Virome analysis of transfusion recipients reveals a novel human virus that shares genomic features with hepaciviruses and pegiviruses. MBio. 2015;6:e0146615. DOIPubMed
  22. Chevreux  B, Pfisterer  T, Drescher  B, Driesel  AJ, Müller  WEG, Wetter  T, et al. Using the miraEST assembler for reliable and automated mRNA transcript assembly and SNP detection in sequenced ESTs. Genome Res. 2004;14:114759. DOIPubMed
  23. Tokarz  R, Williams  SH, Sameroff  S, Sanchez Leon  M, Jain  K, Lipkin  WI. Virome analysis of Amblyomma americanum, Dermacentor variabilis, and Ixodes scapularis ticks reveals novel highly divergent vertebrate and invertebrate viruses. J Virol. 2014;88:1148092. DOIPubMed
  24. Vandegrift  KJ, Kapoor  A. The ecology of new constituents of the tick virome and their relevance to public health. Viruses. 2019;11:E529. DOIPubMed
  25. Kumar  S, Stecher  G, Tamura  K. MEGA7: molecular evolutionary genetics analysis, version 7.0 for bigger datasets. Mol Biol Evol. 2016;33:18704. DOIPubMed
  26. Le  SQ, Gascuel  O. An improved general amino acid replacement matrix. Mol Biol Evol. 2008;25:130720. DOIPubMed
  27. Kapoor  A, Li  L, Victoria  J, Oderinde  B, Mason  C, Pandey  P, et al. Multiple novel astrovirus species in human stool. J Gen Virol. 2009;90:296572. DOIPubMed
  28. de Souza  WM, Dennis  T, Fumagalli  MJ, Araujo  J, Sabino-Santos  G Jr, Maia  FGM, et al. Novel parvoviruses from wild and domestic animals in Brazil provide new insights into parvovirus distribution and diversity. Viruses. 2018;10:E143. DOIPubMed
  29. Arbetman  AE, Lochrie  M, Zhou  S, Wellman  J, Scallan  C, Doroudchi  MM, et al. Novel caprine adeno-associated virus (AAV) capsid (AAV-Go.1) is closely related to the primate AAV-5 and has unique tropism and neutralization properties. J Virol. 2005;79:1523845. DOIPubMed
  30. Ng  TFF, Willner  DL, Lim  YW, Schmieder  R, Chau  B, Nilsson  C, et al. Broad surveys of DNA viral diversity obtained through viral metagenomics of mosquitoes. PLoS One. 2011;6:e20579. DOIPubMed
  31. de Souza  WM, Fumagalli  MJ, de Araujo  J, Sabino-Santos  G Jr, Maia  FGM, Romeiro  MF, et al. Discovery of novel anelloviruses in small mammals expands the host range and diversity of the Anelloviridae. Virology. 2018;514:917. DOIPubMed
  32. Maia  FGM, de Souza  WM, Sabino-Santos  G Jr, Fumagalli  MJ, Modha  S, Murcia  PR, et al. A novel polyomavirus in sigmodontine rodents from São Paulo State, Brazil. Arch Virol. 2018;163:29135. DOIPubMed
  33. Hansen  TA, Fridholm  H, Frøslev  TG, Kjartansdóttir  KR, Willerslev  E, Nielsen  LP, et al. New type of papillomavirus and novel circular single stranded DNA virus discovered in urban Rattus norvegicus using circular DNA enrichment and metagenomics. PLoS One. 2015;10:e0141952. DOIPubMed
  34. Kapoor  A, Simmonds  P, Scheel  TK, Hjelle  B, Cullen  JM, Burbelo  PD, et al. Identification of rodent homologs of hepatitis C virus and pegiviruses. MBio. 2013;4:e0021613. DOIPubMed
  35. Smith  DB, Becher  P, Bukh  J, Gould  EA, Meyers  G, Monath  T, et al. Proposed update to the taxonomy of the genera Hepacivirus and Pegivirus within the Flaviviridae family. J Gen Virol. 2016;97:2894907. DOIPubMed
  36. Reuter  G, Boros  Á, Mátics  R, Kapusinszky  B, Delwart  E, Pankovics  P. Divergent hepatitis E virus in birds of prey, common kestrel (Falco tinnunculus) and red-footed falcon (F. vespertinus), Hungary. Infect Genet Evol. 2016;43:3436. DOIPubMed
  37. Wu  Z, Lu  L, Du  J, Yang  L, Ren  X, Liu  B, et al. Comparative analysis of rodent and small mammal viromes to better understand the wildlife origin of emerging infectious diseases. Microbiome. 2018;6:178. DOIPubMed
  38. Yinda  CK, Ghogomu  SM, Conceição-Neto  N, Beller  L, Deboutte  W, Vanhulle  E, et al. Cameroonian fruit bats harbor divergent viruses, including rotavirus H, bastroviruses, and picobirnaviruses using an alternative genetic code. Virus Evol. 2018;4:vey008. DOIPubMed
  39. McMullan  LK, Albariño  CG, Ksiazek  TG, Nichol  ST, Spiropoulou  CF. Complete genome sequences of a hantavirus isolate from New York. Genome Announc. 2018;6:e00188-18. DOIPubMed
  40. Sakamoto  JM, Ng  TFF, Suzuki  Y, Tsujimoto  H, Deng  X, Delwart  E, et al. Bunyaviruses are common in male and female Ixodes scapularis ticks in central Pennsylvania. PeerJ. 2016;4:e2324. DOIPubMed
  41. Peters  CJ. Emerging infections: lessons from the viral hemorrhagic fevers. Trans Am Clin Climatol Assoc. 2006;117:18996, discussion 196–7.PubMed
  42. Fernando  R, Capone  D, Elrich  S, Mantovani  R, Quarles  L III, D’Amato  A, et al. Infection with New York orthohantavirus and associated respiratory failure and multiple cerebral complications. Emerg Infect Dis. 2019;25:12413. DOIPubMed
  43. Kreuder Johnson  C, Hitchens  PL, Smiley Evans  T, Goldstein  T, Thomas  K, Clements  A, et al. Spillover and pandemic properties of zoonotic viruses with high host plasticity. Sci Rep. 2015;5:14830. DOIPubMed
  44. Pandit  PS, Doyle  MM, Smart  KM, Young  CCW, Drape  GW, Johnson  CK. Predicting wildlife reservoirs and global vulnerability to zoonotic Flaviviruses. Nat Commun. 2018;9:5425. DOIPubMed
  45. Alexander  KA, Lewis  BL, Marathe  M, Eubank  S, Blackburn  JK. Modeling of wildlife-associated zoonoses: applications and caveats. Vector Borne Zoonotic Dis. 2012;12:100518. DOIPubMed
  46. Ostfeld  RS, Brisson  D, Oggenfuss  K, Devine  J, Levy  MZ, Keesing  F. Effects of a zoonotic pathogen, Borrelia burgdorferi, on the behavior of a key reservoir host. Ecol Evol. 2018;8:407483. DOIPubMed
  47. Phan  TG, Kapusinszky  B, Wang  C, Rose  RK, Lipton  HL, Delwart  EL. The fecal viral flora of wild rodents. PLoS Pathog. 2011;7:e1002218. DOIPubMed
  48. Sadeghi  M, Altan  E, Deng  X, Barker  CM, Fang  Y, Coffey  LL, et al. Virome of > 12 thousand Culex mosquitoes from throughout California. Virology. 2018;523:7488. DOIPubMed




Suggested citation for this article: Kumar A, Vandegrift KJ, Sharma H, Murthy S, Kramer LD, Ostfeld R, et al. Virome analysis for detection of segmented flaviviruses in wild rodents, Pennsylvania, USA. Emerg Infect Dis. 2020 Aug [date cited].

DOI: 10.3201/eid2608.190986

Original Publication Date: June 29, 2020

1These authors contributed equally to this work.

Table of Contents – Volume 26, Number 8—August 2020


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Amit Kapoor, Abigail Wexner Research Institute at Nationwide Children’s Hospital, 700 Children’s Dr, Columbus, OH 43205, USA

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