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Volume 28, Number 3—March 2022

Transovarial Transmission of Heartland Virus by Invasive Asian Longhorned Ticks under Laboratory Conditions

Wilson R. Raney, Josiah B. Perry, and Meghan E. HermanceComments to Author 
Author affiliation: University of South Alabama College of Medicine, Mobile, Alabama, USA

Cite This Article


We demonstrated experimental acquisition and transmission of Heartland bandavirus by Haemaphysalis longicornis ticks. Virus was detected in tick salivary gland and midgut tissues. A total of 80% of mice exposed to 1 infected tick seroconverted, suggesting horizontal transmission. H. longicornis ticks can transmit the virus in the transovarial mode.

The Asian longhorned tick, Haemaphysalis longicornis, is an ixodid tick native to Southeast Asia that was reported in the United States during 2017 and has since been found in 17 states (1,2). In its native range, this tick is the main vector of Dabie bandavirus (3) (formerly severe fever with thrombocytopenia syndrome virus), the agent that causes severe human illnesses characterized by high fever, thrombocytopenia, leukopenia, and multiorgan dysfunction (4).

Dabie bandavirus is closely related genetically to Heartland bandavirus (HRTV) (5), an emerging North American virus reported during 2012 after 2 men in Missouri, USA, showed febrile illness with fatigue, thrombocytopenia, and leukopenia after exposure to ticks (6). Because the current geographic range and the predicted range expansion of invasive H. longicornis ticks overlap considerably with human cases of HRTV, including Missouri (7,8), this study was designed to assess the ability of this invasive tick species to maintain and transmit HRTV.

The Study

Figure 1

Detection of Heartland virus (HRTV) RNA by real-time, quantitative reverse transcription PCR reaction of HRTV-injected Haemaphysalis longicornis ticks. Ticks were dissected at 14, 21, 28, and 40 dpi. Tick organs were screened individually. Viral load data are expressed as FFU equivalents per microgram of RNA after normalization to a standard curve. Data were not normally distributed and are presented as medians with interquartile ranges. Statistical significance was determined by using Kruskal-Wallis tests followed by the Dunn test. Limit of detection was ≈10 FFU equivalents/μg RNA. *p<0.05. CAR, carcass; dpi, days postinjection; FFU, focus-forming units; MG, midgut; SG, salivary glands.

Figure 1. Detection of Heartland virus (HRTV) RNA by real-time, quantitative reverse transcription PCR reaction of HRTV-injected Haemaphysalis longicornisticks. Ticks were dissected at 14, 21, 28, and 40 dpi. Tick...

We selected 74 female H. longicornis ticks from an HRTV-free colony into experimental and control groups. We microinjected 50 ticks with 300 focus-forming units of HRTV into the anal pore and 24 ticks with an equivalent volume of Dulbecco modified Eagle medium into the anal pore (Appendix). We dissected ticks at 14, 21, 28, and 40 days postinjection (dpi) and collected the salivary glands, midgut, and carcass of each tick. We screened tick samples for HRTV RNA by using quantitative reverse transcription PCR (qRT-PCR) (Table 1; Figure 1). No samples taken from media-injected ticks screened positive for HRTV (Table 1). For virus-injected ticks, HRTV RNA titers followed a general trend across each organ, and titers peaked at 21 dpi (Figure 1).

To screen HRTV-microinjected ticks for infectious virions, we collected ticks at 14, 21, 28, and 40 dpi and individually homogenized them. We cultured tick homogenates in triplicate on Vero E6 cells, and titered infectious virus by using a focus-forming assay (FFA). All ticks from each time point produced foci, indicating the presence of infectious virions in the tick body at each interval (Table 1).

We selected an additional 26 female H. longicornis ticks to evaluate horizontal transmission of HRTV to BALB/c mice. We microinjected 16 ticks with HRTV and the remaining 10 with Dulbecco modified Eagle medium. At 40 dpi, mice were infested with the microinjected ticks at a ratio of 1 tick/mouse. Five of the HRTV-injected ticks and 5 medium-injected ticks attached and fed on the mice to repletion. After feeding was complete, we removed engorged ticks and housed them individually to aid oviposition. We monitored mice daily for clinical signs of disease. We collected blood from the mice at −1, 7, and 14 days after tick attachment. Mice were subjected to necropsy at 28 days after attachment, and we collected liver, spleen, kidney, brain, blood, and testis samples. We screened blood and organ samples for HRTV RNA by qRT-PCR. No HRTV RNA was detected in any blood or organs collected from the mice.

We screened serum from the terminal blood samples to determine whether mice seroconverted relative to HRTV. We assayed each serum sample on 2 independent occasions. In brief, we assayed diluted serum samples by using HRTV-infected Vero E6 cells as antigens. Four of the 5 mice fed upon by a single HRTV-injected tick were positive for HRTV-specific antibodies. We detected antibodies up to a serum dilution of 1:1,600 for 3 mice and 1:800 for 1 mouse. None of the 5 mice fed upon by media-injected ticks were positive for HRTV-specific antibodies. Likewise, none of the age-matched, sex-matched, preimmune mouse serum demonstrated an antibody response to HRTV.

Figure 2

Scatter plot demonstrating detection of Heartland virus (HRTV) by real-time, quantitative reverse transcription PCR. Data were not normally distributed and are presented as medians with interquartile ranges. Fed female carcasses, egg pools, and larvae pools were screened for viral RNA. Egg pools and larvae pools were composed of 50 eggs or larvae per pool. Limit of detection was ≈10 FFU equivalents/μg RNA. FFU, focus-forming units.

Figure 2. Scatter plot demonstrating detection of Heartland virus (HRTV) by real-time, quantitative reverse transcription PCR. Data were not normally distributed and are presented as medians with interquartile ranges. Fed female carcasses,...

After each fed female tick completed oviposition, we removed the fed female carcass from the egg mass and homogenized the carcass. We screened the carcasses for HRTV RNA by qRT-PCR, and 5/5 HRTV-injected female carcasses were positive for HRTV RNA (Table 2; Figure 2). The media-injected fed female carcasses were negative for HRTV. We also removed 3 pools of 50 eggs/egg mass to screen for HRTV RNA. All 15 egg pools from HRTV-injected ticks were positive for HRTV RNA (Table 2; Figure 2). Egg pools from the media-injected ticks had no HRTV RNA.

We repeated this analysis for pools of larvae (4 pools of 50 larvae derived from each fed female) after hatching. All larvae clutches derived from HRTV-injected females were positive for HRTV RNA. To screen for infectious virions in larvae, we homogenized pools of 150 larvae from each clutch and cultured them on Vero E6 cells. We titered the infectious virus by using FFA, and all 5 clutches derived from HRTV-injected females were positive for infectious HRTV (Table 2).


We demonstrated experimental acquisition and transmission of HRTV by H. longicornis ticks after microinjection of the anal pore with HRTV. Although not a natural route of virus acquisition for ticks, microinjection of the anal pore is an established and reproducible procedure that delivers specific quantities of virus into the alimentary canal of the tick, the first organ system that virus contacts in naturally infected ticks (9). Microinjected ticks showed viral RNA titers peaking at 21 dpi in salivary glands, midguts, and carcasses, suggesting that HRTV replication took place within these organs between 14 and 21 dpi.

Maintenance of infectious HRTV virions for several weeks after microinjection suggests that an artificially infected tick is capable of transmitting HRTV to vertebrate hosts on which it feeds long after viral acquisition. Although the mice exposed to HRTV-infected ticks did not show clinical signs of disease and viral RNA was not detected in any mouse tissues, the absence of disease in these immunocompetent mice was expected; previously, only immunocompromised Ag129 mice have shown detectable viremia, clinical signs of HRTV infection, and death (10). Seroconversion of 4/5 mice exposed to an individual HRTV-infected H. longicornis tick suggests horizontal transmission of HRTV. Future studies should confirm the presence of infectious virions in tick saliva to eliminate the possibility of seroconversion caused by transmission of noninfectious HRTV antigens during tick feeding.

We also showed transovarial transmission of HRTV in H. longicornis ticks by detection of HRTV RNA in eggs and larvae derived from HRTV-infected mother ticks. Furthermore, we demonstrated the presence of infectious virions in larvae after hatching. The North American strain of the tick is parthenogenetic, a foremost public health concern because 1 female can reproduce asexually to establish and sustain local populations (11). Because H. longicornis ticks are a 3-host tick and a host generalist (12), the possibility of invasive H. longicornis ticks acquiring HRTV by cofeeding with infected ticks or by feeding on a viremic host further highlights the potential of the tick to efficiently disseminate the virus. This distinction becomes more crucial because the tick can withstand a wide range of climates (7,13). Further studies should be conducted to demonstrate whether the tick can transmit HRTV during co-feeding with other ticks because this would be a major factor in promoting the environmental spread of the virus.

The predicted spread of H. longicornis ticks in the United States shares a geographic range with states in which HRTV has already been reported in Amblyomma americanum ticks and wildlife (7,8,14). The introduction of a new vector species could amplify transmission in natural foci, resulting increased HRTV disease cases in humans.

Mr. Raney is a research technologist in the Laboratory of Infectious Diseases at the College of Medicine, University of South Alabama, Mobile, AL. His research interests include tick-borne viruses and tick‒host‒virus interactions.



We thank the Michele Schuler, Leigh Ann Wiggins, and Hannah Bryant for assistance with animal experiments and animal husbandry; and Michael Levin for providing the initial H. longicornis ticks (distributed by BEI Resources, that seeded our in-house colony of ticks used in this study.

This study was supported by the University of South Alabama College of Medicine and the National Institute of Allergy and Infectious Diseases, National Institutes of Health (award no. R21AI163693).



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Cite This Article

DOI: 10.3201/eid2803.210973

Original Publication Date: February 07, 2022

Table of Contents – Volume 28, Number 3—March 2022

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

Meghan E. Hermance, Department of Microbiology and Immunology, University of South Alabama College of Medicine, 610 Clinic Dr, Mobile, AL 36688, USA

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Page created: December 08, 2021
Page updated: February 21, 2022
Page reviewed: February 21, 2022
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