- Open Access
Evaluating the mosquito host range of Getah virus and the vector competence of selected medically important mosquitoes in Getah virus transmission
Parasites & Vectors volume 16, Article number: 99 (2023)
The Getah virus (GETV) is a mosquito-borne Alphavirus (family Togaviridae) that is of significant importance in veterinary medicine. It has been associated with major polyarthritis outbreaks in animals, but there are insufficient data on its clinical symptoms in humans. Serological evidence of GETV exposure and the risk of zoonotic transmission makes GETV a potentially medically relevant arbovirus. However, minimal emphasis has been placed on investigating GETV vector transmission, which limits current knowledge of the factors facilitating the spread and outbreaks of GETV.
To examine the range of the mosquito hosts of GETV, we selected medically important mosquitoes, assessed them in vitro and in vivo and determined their relative competence in virus transmission. The susceptibility and growth kinetics of GETVs in various mosquito-derived cell lines were also determined and quantified using plaque assays. Vector competency assays were also conducted, and quantitative reverse transcription-PCR and plaque assays were used to determine the susceptibility and transmission capacity of each mosquito species evaluated in this study.
GETV infection in all of the investigated mosquito cell lines resulted in detectable cytopathic effects. GETV reproduced the fastest in Culex tritaeniorhynchus- and Aedes albopictus-derived cell lines, as evidenced by the highest exponential titers we observed. Regarding viral RNA copy numbers, mosquito susceptibility to infection, spread, and transmission varied significantly between species. The highest vector competency indices for infection, dissemination and transmission were obtained for Cx. tritaeniorhynchus. This is the first study to investigate the ability of Ae. albopictus and Anopheles stephensi to transmit GETV, and the results emphasize the role and capacity of other mosquito species to transmit GETV upon exposure to GETV, in addition to the perceived vectors from which GETV has been isolated in nature.
This study highlights the importance of GETV vector competency studies to determine all possible transmission vectors, especially in endemic regions.
The Getah virus (GETV) is a mosquito-borne virus and a member of the Alphavirus genus, one of the two genera that comprise the Togaviridae family (the other being the genus Rubivirus) . Like other members of this genus, GETV has an icosahedral capsid and a positive-sense, single-stranded RNA with an 11,598-nucleotide-long genome that mimics messenger RNA (mRNA) . There are > 30 species in the Alphavirus genus, which can be further divided into seven sera-complexes, including the Barmah Forest, Middleburg, Ndumu, Venezuelan equine encephalitis, Western equine encephalitis and Semliki Forest virus (SFV) serogroups [2,3,4,5]. GETV belongs to the SFV serogroup  and is geographically restricted to the Old World, with a widespread distribution across Asia [7,8,9,10,11,12].
GETV is related to other arthritogenic alphaviruses, such as Chikungunya virus (CHIKV), O’nyong’nyong virus and the closely related Ross River virus (RRV) (all pathogenic viruses in humans) . It has been considered to represent a significant risk in veterinary medicine because of the clinical symptoms it elicits, including nasal discharge, fever, rash, edema, lymphadenopathy in horses and abortion in pigs [14, 15]. Despite being closely related to RRV, which is pathogenic to humans , the consequences of GETV infection in humans remain unclear [17, 18]. In addition to the increased number of new GETV strains being isolated from insects and animals [17, 19], seroepidemiological findings from a number of studies suggest human exposure, thus highlighting the risks of these viruses to public health, especially in the context of emerging strains with the potential for virulence [17, 20,21,22].
GETV was first isolated from Culex gelidus mosquitoes in Malaysia in 1955  and subsequently found to be endemic to a number of regions where several disease outbreaks were reported in domestic animals, including horses [12, 24], pigs [25, 26], red pandas , wild blue foxes  and cattle . Outbreaks of GETV have been reported in Japan [24, 25, 30, 31], India  and mainland China [26, 28, 29]; all were linked to domestic animal infections without clear information on the vectors involved. GETV strains have also been detected in a variety of other mosquito species, such as Culex tritaeniorhynchus, Culex vishnui, Culex fuscocephala, Armigeres subalbatus, Anopheles vagus, Anopheles sinensis, Aedes albopictus, Aedes aegypti, Aedes vexans nipponii, Mansonia annulifera, as well as in some unspecified mosquito species [32, 33]. However, it is still unknown how much these insects contribute to GETV transmission; this lack of information is especially relevant for Anopheles mosquitoes, which have the ability to adapt to new and urban dwellings. Anopheles stephensi mosquitoes are highly endophilic and anthropophilic and have been determined to be susceptible to infection by CHIKV . It is an urban-dwelling species that is wide-spread in Southeast Asia and the Arabian Peninsula . The introduction of these mosquitoes to new areas is partially driven by their resistance to several classes of insecticides and by increases in international travel, factors which make effective control measures more difficult to implement and faciliate spread to newer areas [35, 36]. Although the susceptibility of An. stephensi to GETV infection has never been determined, the high abundance of this mosquito species and related species within the genus can represent a potential risk in terms of GETV transmission. Culex tritaeniorhynchus and Ar. subalbatus are two mosquito species that are widely distributed across Southeast Asia, and multiple isolates of GETV have been identified in these mosquito species , especially Cx. tritaeniorhynchus, leading to suggestions that this latter mosquito species may be the principal vector of transmission among farm animals in Japan . Aedes albopictus, aside from being highly invasive, is also of global concern due to its vectorial competence in transmitting many arboviruses, including dengue virus in Asia . Thus, the abundance and/or high distribution of these mosquito species in areas where GETV is known to circulate, the susceptibility of these mosquito species to GETV and their role in the spread of medically important arboviruses need to be further investigated.
In this context, it is of increasing importance to expand the scope of assessing vector competency to include indigenous mosquito species with the potential to spread GETV in areas endemic to GETV (owing to increased international travel and altering environmental conditions) [35, 36]. Wild boars, horses, and pigs are examples of putative amplifying hosts for GETV; nonetheless, the persistence of GETV outbreaks in specific areas is contingent upon the presence of effective vectors (such as mosquitoes). This further poses a challenge in characterizing the importance of GETV mosquito vectors in nature and forecasting future outbreaks based on the seasonal activity of these mosquitoes.
Prior studies have used mosquito-derived cell culture systems to address the above challenges by analyzing arbovirus infection and replication as a tractable alternative to current in vivo models for assessing vector competencies [39,40,41]. These methods have transformed arbovirus studies and have provided deeper insights into virus susceptibility and virus-vector host interactions [41, 42]. For example, C6/36 (derived from Ae. albopictus), MSQ43 (derived from An. stephensi) and AeAe-GH98 (derived from Ae. aegypti) cells are now used as cell culture systems for the propagation of many arboviruses [39,40,41]. Other cell lines, in addition of mosquito cell lines, that have previously been used for the propagation of GETV include CPK (pig kidney), HmLu-1 (hamster lung), Vero (African green monkey kidney) and BHK-21 (hamster kidney) [43, 44]. Until now, the isolation and propagation of GETV have been limited to C6/36 cells [8, 45, 46] with little to no involvement of other mosquito-derived cultured cells. In the present study, we examined the suitability of several mosquito cell lines, namely MSQ43 (derived from An. stephensi), NIID-CTR (derived from Cx. tritaeniorhynchus) and Ar-3 (derived from Ar. subalbatus), in propagating GETV. We also performed an in vivo experiment to evaluate the vector competency of Cx. tritaeniorhynchus, An. stephensi, and Ae. albopictus for transmitting GETV.
Cell lines and GETV strain
Four mosquito-derived cell lines and one mammalian-derived cell line were used in this study. Culex tritaeniorhynchus-derived NIID-CTR cells  and Ar. subalbatus-derived Ar-3 cells  were maintained in Varma-Pudney (VP12) medium supplemented with 10% heat-inactivated fetal bovine serum (FBS; Biowest, Nuaillé, France) and penicillin–streptomycin solution (100 U/ml; FUJIFILM Wako Pure Chemical Corp., Osaka, Japan). Anopheles stephensi-derived MSQ43 (BEI Resources, Manassas, VA, USA)  and Ae. albopictus-derived C6/36 cells (European Collection of Authenticated Cell Cultures, Darmstadt, Germany)  were cultured in Eagle’s minimum essential medium (MEM) supplemented with 10% heat-inactivated FBS and 2% nonessential amino acids (FUJIFILM Wako Pure Chemical Corp.). One mammalian cell line, Vero cells, derived from the African green monkey kidney (Japanese Collection of Research Bioresources Cell Bank, Osaka, Japan), was maintained in MEM supplemented with 10% heat-inactivated FBS. Mammalian and mosquito cell cultures were adapted to in vitro conditions with 5% CO2 and temperatures of 37 °C and 28 °C, respectively, except for NIID-CTR cells, which were incubated at 25 °C. The four mosquito-derived cell lines were used for the in vitro growth kinetics study only. Mammalian-derived Vero cells were used for virus stock propagation (prior to in vitro and in vivo experiments) and viral quantification (plaque assay).
The GETV strain used in this study was the 12IH26 strain, isolated from Cx. tritaeniorhynchus mosquitoes collected in Isahaya City, Nagasaki Prefecture, Japan, in September 2012 (GenBank accession no. LC152056) . GETV 12IH26, in addition to being recently isolated by our laboratory  and being readily available, may be representative of the current and possible circulating strain among farm animals in Japan, as evidenced by recent studies .
Infection of mosquito-derived cell cultures
A monolayer of 1.0 × 105 cells was seeded in a 25-cm2 cell culture flask and incubated overnight at 28 °C, 5% CO2. The adhered cells were then inoculated with GETV 12IH26 at a multiplicity of infection (MOI) of 0.01 and incubated for 1 h. The cells and cell culture supernatants were harvested at 0, 12, 24, 48, 72, 96 and 120 h post-infection (hpi) and stored at − 80 °C until analysis. The virus titers in cells were determined from freeze-thawed lysates and cell supernatants using the plaque assay method . A plot of virus titers against time was represented by linear regression curves and bar graphs. All samples were run in triplicate with controls (supernatants from mock-infected cell cultures). The effect of GETV infection on cultured cells was determined via microscopy and a Trypan blue-based cell viability test using an automated cell counter (Countess™ II Automated Cell Counter; Thermo Fisher Scientific, Waltham, MA, USA).
Infection of mosquitoes
Mosquito infections were performed in a BSL-2 insectary at the National Institute of Infectious Diseases, Tokyo, Japan, as previously reported [52, 53]. Briefly, 7- to 14-day-old female mosquitoes were starved overnight and fed defibrinated rabbit blood (Nippon Bio-Supp. Center, Tokyo, Japan) supplemented with 3 mM ATP (Sigma-Aldrich, St. Louis, MO, USA) containing 1.0 × 106 PFU (plaque-forming unit)/ml GETV. Feeding was performed using an artificial membrane feeding system for blood-sucking insects (Hemotek™ 5W1; Hemotek Ltd., Blackburn, UK). Mosquitoes were allowed to feed for 1 h, and only fully engorged mosquitoes were included in subsequent experiments and analyses. Fully engorged females were kept at 27 ± 0.5 °C, and a 10% sugar solution was provided ad libitum; the mosquitoes were maintained for several days before the time points for salivation and dissection.
Salivation and mosquito dissection
Mosquito salivation and dissection were performed at 5, 10, and 15 days post-infection (dpi) following methods described in previous studies [52, 53]. Briefly, the wings and legs of CO2-anesthetized mosquitoes were clipped for immobilization. Salivation was induced by inserting the proboscises of the mosquitoes into 10-µl pipette tips containing 10 µl of FBS. The mosquitoes were allowed to salivate for 1 h prior to dissection. Harvested saliva was collected in tubes containing 100 µl MEM that contained 2% FBS, 2% Amphotericin B (Thermo Fisher Scientific) and 2% penicillin–streptomycin. The mosquitoes were dissected into the thorax/abdomen and head/wings/legs regions, and these regions were stored at − 80 °C until use.
RNA extraction and virus quantification using quantitative reverse transcription-PCR and plaque assays
RNA was extracted using a Nucleospin RNA extraction kit (Macherey–Nagel, Dueren, Germany) according to the manufacturer’s instructions, with slight modifications. Specifically, prior to extraction, the mosquito body parts were homogenized in a TissueLyser II flexible bead mill (Qiagen, Hilden, Germany) to which RA1 Buffer (Macherey–Nagel) supplemented with 1% beta-mercaptoethanol (FUJIFILM Wako Pure Chemical Corp.) had already been added. The samples were then centrifuged at 12,000 rpm for 3 min; the remaining RNA extraction steps were conducted following the manufacturer’s instructions. The filtered homogenate was subjected to DNase treatment before the RNA was eluted with 20 μl of RNase-free water.
After RNA extraction, quantitative reverse transcription PCR (qRT-PCR) was used to quantify viral copy numbers. Information on the primers and probes used in this study is given in Table 1. Briefly, RNA samples were mixed with Taq-Man Fast Virus 1-Step Master Mix (Thermo Fisher Scientific), GETV primers (forward and reverse, 10 μM each) and GETV probes (10.1 μM), and then quantified by running on a PikoReal RT-PCR System (version 2.2.; Thermo Fisher Scientific). The qRT-PCR cycling conditions were: 1 cycle at 50 °C for 5 min and 95 °C for 20 s, followed by 35 cycles at 95 °C for 3 s and 60 °C for 30 s. Cq values > 30 were regarded as a negative result, as shown in Additional file 1: Figure S1.
Plaque assays were used to quantify the initial viral stock and mosquito saliva samples. Vero cells were used for plaque assay quantification, as described previously . Briefly, Vero cells were seeded into 24-well plates overnight at a density of 2 × 105 cells/well. A 100-μl aliquot of 1:100 diluted supernatant samples prepared in MEM was added to each well. After incubation for 1 h at 37 °C, the inoculum, MEM supplemented with 1% methylcellulose and 2% FBS were added to each well. The cell setup was further incubated at 37 °C for 3 days, following which the cells were fixed with 4% paraformaldehyde and stained with methylene blue for plaque visualization and PFU estimation.
Vector competency evaluation points and statistical analysis
The infection rate (IR), dissemination rate (DR) and transmission rate (TR) of all three sample groups (5, 10 and 15 dpi) were computed. The IR was considered to be the proportion of virus-positive mosquito bodies (head-thorax) to fed females ([number of GETV-positive females/total number of fully-fed females]) × 100; the DR was considered to be the proportion of virus-positive mosquito carcasses (head-wings-legs) to virus-positive bodies ([GETV-positive in the carcasses, i.e. head-wings-legs/total number GETV-positive females] × 100). The TR was considered to be the proportion of virus-positive saliva to virus-positive carcasses ([GETV-positive saliva/ GETV-positive carcasses]).
GraphPad Prism software (version 7; GraphPad Software, San Diego, CA, USA) was used for all statistical analyses. Statistical significance was computed between tabulated data points using the Kruskal–Wallis test corrected with Bonferroni’s method and Fisher’s exact test. A P-value < 0.05 was considered to be statistically significant. Results are presented as the mean ± standard deviation (SD) .
GETV growth rate in vitro is species-dependent
GETV-infected NIID-CTR (Cx. tritaeniorhynchus), C6/36 (Ae. albopictus), MSQ43 (An. stephensi) and Ar-3 (Ar. subalbatus) cells and their respective culture supernatants were collected at 0, 12, 24, 48, 72, 96 and 120 hpi. All four cell lines were found to be susceptible to GETV infection (Fig. 1). In general, the virus titers in the cells were inversely proportional to those in the supernatants in all cell lines, with the exception of NIID-CTR cells (Figs. 1, 2). In terms of GETV propagation efficiency, C6/36 cells were the most efficient cell line for propagating GETV, whereas MSQ43 cells were the least efficient (Fig. 1; Table 2). Similarly, GETV reached the stationary phase of growth within 48 hpi in C6/36 and Ar-3 cells, whereas it took 96 hpi to reach the stationary phase in NIID-CTR and MSQ43 cells (Fig. 1; Table 2). The GETV titers in C6/36 and Ar-3 cells at the plateau phase were 7.87 × 108 and 5.03 × 105 PFU/ml, respectively (Table 2). The highest virus titers were recorded in the extracellular fractions of each cell line over the period 0–120 hpi (Fig. 2). GETV titers in the extracellular fractions generally showed no significant difference compared to the freeze-thawed cell lysates between cell lines despite variations in the peaks at different time points, except in C6/36 (at 96 hpi) and MSQ43 cells (at 120 hpi) (p = 0.1467, Fisher’s exact test) (Fig. 2). The virus titers of freeze-thawed lysates of C6/36, NIID-CTR and Ar-3 cells peaked above the initial inoculum titer (103 PFU/ml, 0 hpi) after 12 hpi (105 PFU/ml, Fig. 2a–c). However, MSQ43 cells showed no significant increase in virus titer from the initial inoculum of 103 PFU/ml after 12 hpi (Fig. 2d).
GETV proliferation induces the cytopathic effect and decreases cell proliferation
The morphological alterations that occurred in the cells were examined, and pictures were taken of the GETV-induced cytopathic effect (CPE). Mock-infected cells were used as the control, and the control cells were compared with GETV-infected cells (Additional file 2: Figure S2). An apparent CPE was observed in GETV-infected C6/36, NIID-CTR, Ar-3 and MSQ43 cells after 48, 72, 72 and 72 hpi, respectively (Additional file 2: Figure S2g, r, bb, ll), with the appearance of some rounded, aggregated and detached cells. An obvious CPE was the decrease in the number of cells, especially in C6/36 and MSQ43 cells at 72 hpi (Additional file 2: Figure S2,h, ll) together with an increase in cell distance. The most severe GETV-induced CPE was observed in MSQ43 cells (120 hpi); in contrast, the least severe CPE was observed in NIID-CTR cells. Characteristic compact cell aggregations were missing in the GETV-infected Ar-3 cells . The mock-infected cells from each cell line demonstrated significant overgrowth, with sloughing and stacking of the cell monolayers, when observed up to 120 hpi (Additional file 2: Figure. S2). This observation was confirmed by estimating the cell population using a Trypan blue exclusion assay (Fig. 3a–d). This assays showed that cell death in GETV-infected cells corresponded to a loss of monolayer integrity over time, with the percentage of viable cells dropping from a brief period of proliferation (Fig. 3e–h), consistent with the cytolysis observed via microscopic analysis at each time point (Additional file 2: Figure S2). A significant decrease in MSQ43 cell proliferation in cell culture was observed following GETV infection (P = 0.05) compared to C6/36, NIID-CTR, and Ar-3 cells. In addition, NIID-CTR cells were more resistant to GETV-induced CPE (Fig. 3e–h) despite the relatively high permissiveness of these cells to GETV propagation (Fig. 1).
GETV specificity in mosquito vectors
A total of 141 Cx. tritaeniorhynchus, 146 An. stephensi and 51 Ae. albopictus mosquitoes were evaluated. The feeding rates in these mosquito colonies were 78% (141/180), 92% (156/170), and 43% (51/120) for Cx. tritaeniorhynchus, An. stephensi and Ae. albopictus, respectively. All three tested species were susceptible to GETV infections in their midgut, with the infection established within 5 days of virus acquisition (Table 3; Fig. 4a–c). Aedes albopictus was the most susceptible of the four mosquito species to midgut infection, with a combined IR of 96%, while An. stephensi was the least susceptible, with a combined IR of 57% (Table 3). Further analysis of viral RNA copy numbers within the midgut of each species after virus exposure showed a significant decrease in viral RNA content (P = 0.01, analysis of variance [ANOVA]). In addition, the number of viral RNA copies detected in the midgut of individual mosquitoes per sample decreased with time (Fig. 4a–c). The viral titers in the midgut of Cx. tritaeniorhynchus decreased further, while significantly higher (P < 0.05) GETV RNA copy numbers were recorded in this species compared to An. stephensi and Ae. albopictus (Fig. 4a–c). Based on RNA replication data, Cx. tritaeniorhynchus was the most susceptible to GETV infection with increasing time post-exposure (Fig. 4a).
RNA copy numbers differed significantly among mosquito species during dissemination
The dynamics of GETV dissemination were determined in each mosquito species by measuring the amount of viral RNA in the heads, wings and legs of each individual mosquito evaluated (Fig. 4d–f). Virus dissemination within the mosquito colonies post-infection was consistent with their susceptibility to infection. For example, Cx. tritaeniorhynchus had significantly higher RNA copy numbers at all time points (P = 0.01), which was consistent with the high RNA dissemination recorded with increasing time (Fig. 4d). Generally, there was a decrease in the number of GETV-disseminating individuals and lower GETV RNA titers in An. stephensi and Ae. albopictus (Fig. 4d–f) relative to previous reports where a higher number of GETV-infected individuals and higher GETV RNA titers post-GETV-laced blood meal (Fig. 4a–c) were observed, respectively. Although a combined DR > 80% was recorded for each colony, the highest sensitivity to virus dispersion per number of individuals was recorded among the Ae. albopictus colonies (combined value: 94%, P = 0.351; Table 3), followed by Cx. tritaeniorhynchus and An. stephensi at 90% and 89%, respectively.
Significant differences in the transmission rate between mosquito species
To ascertain their capacity for GETV transmission, the saliva of mosquitoes that showed signs of virus propagation was investigated for the presence of live viruses. The TR was calculated based on the proportion of mosquitoes with saliva that tested positive for virus among those with positive RNA dissemination. The TRs ranged from 30% to 96% over extrinsic incubation periods of 5, 10, and 15 days. In terms of numbers, Cx. tritaeniorhynchus had the highest population to achieve positive TR (74%, 5 dpi; Table 3). The highest titer in GETV-positive individuals (maximum titer: 107 PFU/ml; Fig. 4g) was recorded in An. stephensi despite it having the fewest GETV-positive individuals. Anopheles stephensi also showed the longest extrinsic incubation period to produce detectable viruses in the saliva, at 10 dpi (96%). In terms of combined TR, Cx. tritaeniorhynchus was the colony with the most significant successive transmission (78%, P = 0.001), followed by An. stephensi and Ae. albopictus at 53% and 41%, respectively (Table 3). Live viruses were detected in the saliva of all colonies, indicating the ability of all colonies to produce detectable viruses effectively (Fig. 4g–i). We also observed a decrease in the TR of Ae. albopictus from 60% at 5 dpi to 36% at 15 dpi (Table 3). In contrast with Cx. tritaeniorhynchus and An. stephensi, there was a significantly continuous increase in TR with extension of the extrinsic incubation period (10 and 15 dpi) throughout the testing period (Fig. 4g) compared with TRs in Ae. albopictus. Generally, the lowest virus titers in terms of IR, DR and TR were recorded in the Ae. albopictus colony (Fig. 4). A comparison of the transmission efficiency (TE), which refers to the proportion of GETV-infected mosquitoes exposed to the infectious blood meal that developed detectable virus levels in their saliva, showed that the Cx. tritaeniorhynchus colonies were more efficient (gently increasing slope) in terms of transmission (from 5 to 15 dpi) than the other colonies (Fig. 5).
Beyond RNA detection, only a limited number of studies have investigated the vector range of mosquitoes involved in GETV transmission . Some studies seeking to address this gap were restricted to investigations using Ae. albopictus-derived cells, C6/36 and Cx. tritaeniorhynchus mosquitoes for in vivo analysis due to the importance of these mosquitoes in natural GETV transmission. In the present study, we have shown that the vector compatibility of GETV can be assessed using a range of mosquito-derived cells and demonstrated the competency of these mosquito species for GETV transmission in vivo.
We examined GETV propagation in mosquito cells by comparing the viral titers and CPE in each cell line and discovered that GETV replication was species-specific in vitro. When the cells were exposed to GETV, we found that the cell line NIID-CTR, derived from Cx. tritaeniorhynchus, displayed the most improved susceptibility to GETV replication with minimal pathogenicity, as indicated by the significantly less severe CPE we observed in this cell population. Some arboviruses can interfere with normal cell proliferation by manipulating the subcellular structures of tissues or cells. These viral-induced side effects are frequently characterized by an apparent CPE linked to cell death, such as via apoptosis [55, 56]. Although cytopathology has been observed in some arbovirus-mosquito infections, the apparent but milder CPE observed in NIID-CTR cells suggests that these cells may have evolved to avoid this effect, similar to other host virus-adapted cells [57, 58]. However, it is unclear from the outset whether apoptosis always represents an antiviral response during arbovirus infections in mosquitoes, as we observed that the proliferation of MSQ43 cells was hampered by the replication of GETV. The exposure of C6/36 cells to GETV also resulted in a severe CPE, indicative of the disruptive effect of GETV in these cells. It is important to note that C6/36 cells have defective RNA interference (RNAi) mechanism, implicating the severe CPE observed in these cells when exposed to many other viruses [59,60,61]. As viral titers increased over time, we also observed that the Ar-3 cell line was susceptible to GETV replication in vitro, especially when the virus titer increased from approximately 103 PFU/ml (initial inoculum) to 106 PFU/ml. Despite the evident CPE in Ar-3 cells, the severity of infection was relatively lower than that in C6/36 cells. The Ar-3 cell line, which was derived from Ar. subalbatus, has become an invaluable tool for the titration of some flaviviruses, including the Japanese encephalitis virus, but has a relative insensitivity to another flavivirus, the dengue virus . The detection of GETV in field-sampled Ar. subalbatus mosquitoes [9, 28, 32] and the ability of Ar-3 cell lines to support GETV replication, as shown in the current study, provides us with information on its potentially important role in the study of GETV replication and application in GETV isolation in future surveillance studies.
We also explored the potential tractability of our in vitro findings in vivo and evaluated the vector competency of the three mosquito species. Among the colonies tested, the lowest feeding rate was observed in Ae. albopictus colonies, which had considerable difficulty feeding under laboratory conditions, as has been reported in previous studies using Ae. vexans . In the current study, we compared the IRs of Cx. tritaeniorhynchus (72%) and Ae. albopictus (96%). The IR showed the ability of the virus to escape the midgut infection barrier and to infect the midgut of the mosquito after exposure to the infected blood meal. To our knowledge, this is the first study that has evaluated the transmission capacity of GETV in laboratory-raised Ae. albopictus colonies. Our findings are consistent with previous assessments  that showed a higher IR in Ae. vexans nipponii (100%) than in Cx. tritaeniorhynchus (64%), despite the lower feeding rates among Aedes colonies in the previous study  and the current study. In An. stephensi, a combined IR of 57% was observed. This result is not comparable to that reported in any previously published studies since this is the first reported demonstration of the competency of an Anopheles species, An. stephensi, to GETV. The IR of An. stephensi indicated adequate compatibility with GETV infection in vivo, which corresponds to the ability of An. stephensi-derived MSQ43 cells to support GETV replication, albeit with lower titers under in vitro conditions.
TR represented the ability of the mosquito to harbor infectious virus for transmission, i.e. infection of the salivary gland and escape barriers. In terms of TR, Cx. tritaeniorhynchus and An. stephensi colonies showed a high level of transmissibility, that is, a combined TR of 78% for the former, compared to Ae. albopictus colony. A previous study reported a TR between 0 and 59% in Cx. tritaeniorhynchus, where GETV titers were determined using plaque assays of viruses derived from mosquito saliva secreted into serum-agar or via mouse feeding . However, it is important to note that these disparate TR outcomes may have been influenced by variations in the inoculating titers used in the blood meal of the mosquitoes . In the current study, the combined TRs of 41 and 53% for Ae. albopictus and An. stephensi, respectively, were significantly lower (P < 0.05) than that of Cx. tritaeniorhynchus, which had a combined TR of 78%. A previous study showed that chickens might potentially contract GETV from infected Cx. tritaeniorhynchus mosquitoes but not from Culex pipiens pallens . These results, along with earlier accounts of GETV isolation from Culex mosquitoes [32, 39], led us to speculate that Cx. tritaeniorhynchus mosquitoes are highly susceptible to GETV infection and are able to transmit the virus. Notably, the variable TRs of GETV across Aedes and Culex species have been previously reported in earlier accounts [32, 62], demonstrating differences in TR even among closely related species.
Among the vectors thought to be involved in the transmission of RRV, a human pathogen and an antigen that closely resembles GETV, Culex annulirostris, Aedes vigilax, Aedes notoscriptus and Aedes camptorhynchus mosquitoes have been implicated in RRV transmission in nature . Differences in mosquito species that function as vectors of RRV and GETV, despite the serological closeness of these two viruses, may further explain the variations in vector competence in this study. Culex tritaeniorhynchus is often perceived to be a major vector of GETV transmission in nature, especially in GETV-endemic regions because: (i) GETV isolates have been detected and isolated in this mosquito species; and (ii) this mosquito species shows increased feeding behavior among large domestic animals [65, 66].
Interestingly, the TR and TE of the GETV in An. stephensi (no reports of GETV competence) was much higher than the TR and TE of GETV in Cx. tritaeniorhynchus and Ae. albopictus at 10 dpi and 15 dpi, respectively. The extrinsic incubation time also differed among these three species, highlighting the importance of taking into consideration the time needed for each mosquito to become infectious following exposure to GETV. Furthermore, the salivary glands of Aedes mosquitoes have been suggested to be potentially affected when exposed to SFV infection, which triggers an effective antiviral response that results in an observable CPE . This finding is significant and should be highlighted as it was previously reported that apoptosis was observed in the salivary glands of Ae. albopictus when infected with the Sindbis virus [68, 69], which may affect feeding behavior or reduce virus production in the saliva. In the current study, this phenomenon may explain the low detection rate of infectious viruses in the saliva of Ae. albopictus colonies (TR = 41%), as the immunity within the salivary glands of these mosquito colonies may be refractory to GETV replication or detection compared to colonies of Cx. tritaeniorhynchus and An. stephensi.. The high GETV IR and DR and the ability of the virus to cross the midgut barrier and replicate in the body parts of the mosquito , in both Ae. albopictus and An. stephensi, support the conclusion that GETV can establish infections in the midguts of these species. The low TR of GETV in Ae. albopictus may suggest that the salivary gland barrier is refractory to GETV secretion into the saliva, accounting for the lower TR observed in these species. However, Ae. albopictus was still able to effectively transmit GETV, emphasizing the significance of the midgut infection barrier as an indicator of vector competence. Additional observational studies focusing on the exposure time, anatomical barriers of the mosquitoes, temperature conditions and immunity within mosquito species are necessary to further characterize and ascertain GETV vector competence. It is noteworthy that although An. stephensi mosquitoes have long been regarded as malaria vectors native to the Middle East and South Asia, there have been no reports of GETV detection or transmission perpetuated by An. stephensi. However, since Anopheles species are known to be robust in their ability to adapt to various needs, coupled with the previous isolation of GETV from An. sinensis mosquitoes , the spread of indigenous species to new areas, such as the recent discovery of Anopheles belenrae in Japan , and the potential for emergence of more virulent GETV strains, increases the risk of GETV epidemics.
Our data suggest that, compared to the three other mosquito species examined, Cx. tritaeniorhynchus showed the greatest capacity for the spread and transmission of GETV. The results of this study also confirmed GETV susceptibility in the other mosquito species studied, including Ae. albopictus and An. stephensi. To the best of our knowledge, this is the first study of GETV infection in An. stephensi, and the results highlight the possible role of this species in the GETV transmission cycle. Although GETV growth kinetics in each cell line did not always indicate transmission, the mosquito-derived cell system used in this study offered valuable insights into the susceptibility of mosquito cells and the vector range of GETV. Our aim in the present study was to replicate all in vitro experiments using colonies of the selected mosquitoes; however, current unavailability of a laboratory colony of Ar. subalbatus was a limitation in this study. Importantly, this study provides relevant evidence on the different vector species for GETV transmission, as well as recommendations regarding investigations into the sero-related virus RRV.
Availability of data and materials
The corresponding author can provide the datasets used and/or analyzed during the current investigation upon reasonable request.
Quantitative reverse transcription-PCR
Ribonucleic acid interference
Meshram CD, Agback P, Shiliaev N, Urakova N, Mobley JA, Agback T, et al. Multiple host factors interact with the hypervariable domain of chikungunya virus nsP3 and determine viral replication in cell-specific mode. J Virol. 2018;92:e00838-e918.
Powers AM, Brault AC, Shirako Y, Strauss EG, Kang W, Strauss JH, et al. Evolutionary relationships and systematics of the alphaviruses. J Virol. 2001;75:10118–31.
La Linn M, Gardner J, Warrilow D, Darnell GA, McMahon CR, Field I, et al. Arbovirus of marine mammals: a new alphavirus isolated from the elephant seal louse, Lepidophthirus macrorhini. J Virol. 2001;75:4103–9.
Zacks MA, Paessler S. Encephalitic alphaviruses. Vet Microbiol. 2010;140:281–6.
Travassos da Rosa AP, Turell MJ, Watts DM, Powers AM, Vasconcelos PF, Jones JW, et al. Trocara virus: a newly recognized Alphavirus (Togaviridae) isolated from mosquitoes in the Amazon Basin. Am J Trop Med Hyg. 2001;64:93–7.
Kono Y. Getah virus disease. In: Monath TP, editor. The arboviruses: epidemiology and ecology. Boca Raton: CRC Press; 2019. p. 21–36.
Ksiazek TG, Trosper JH, Cross JH, Basaca-Sevilla V. Isolation of Getah virus from Nueva Ecija Province, Republic of the Philippines. Trans R Soc Trop Med Hyg. 1981;75:312–3.
Morita K, Igarashi A. Oligonucleotide fingerprint analysis of strains of Getah virus isolated in Japan and Malaysia. J Gen Virol. 1984;65:1899–908.
Bryant JE, Crabtree MB, Nam VS, Yen NT, Duc HM, Miller BR. Isolation of arboviruses from mosquitoes collected in northern Vietnam. Am J Trop Med Hyg. 2005;73:470–3.
Turell MJ, O’Guinn ML, Wasieloski LP Jr, Dohm DJ, Lee WJ, Cho HW, et al. Isolation of Japanese encephalitis and Getah viruses from mosquitoes (Diptera: Culicidae) collected near Camp Greaves, Gyonggi Province, Republic of Korea, 2000. J Med Entomol. 2003;40:580–4.
Lvov SD, Gromashevsky VL, Andreev VP, Skvortsova TM, Kondrashina NG, Morozova TN, et al. Natural foci of arboviruses in far northern latitudes of Eurasia. In: Calisher CH, et al., editor. Hemorrhagic fever with renal syndrome, tick-and mosquito-borne viruses. Vienna: Springer; 1990. p. 267–75.
Brown CM, Timoney PJ. Getah virus infection of Indian horses. Trop Anim Health Prod. 1998;30:241–52.
Suhrbier A, Jaffar-Bandjee MC, Gasque P. Arthritogenic alphaviruses–an overview. Nat Rev Rheumatol. 2012;8:420–9.
Nemoto M, Bannai H, Tsujimura K, Kobayashi M, Kikuchi T, Yamanaka T, et al. Getah virus infection among racehorses, Japan, 2014. Emerg Infect Dis. 2015;21:883–5.
Bannai H, Nemoto M, Niwa H, Murakami S, Tsujimura K, Yamanaka T, et al. Geospatial and temporal associations of Getah virus circulation among pigs and horses around the perimeter of outbreaks in Japanese racehorses in 2014 and 2015. BMC Vet Res. 2017;13:187.
Mackenzie JS, Chua KB, Daniels PW, Eaton BT, Field HE, Hall RA, et al. Emerging viral diseases of Southeast Asia and the Western Pacific. Emerg Infect Dis. 2001;7:497–504.
Li XD, Qiu FX, Yang H, Rao YN, Calisher CH. Isolation of Getah virus from mosquitos collected on Hainan Island, China, and results of a serosurvey. Southeast Asian J Trop Med Public Health. 1992;23:730–4.
Lu G, Ou J, Ji J, Ren Z, Hu X, Wang C, et al. Emergence of Getah virus infection in horse with fever in China, 2018. Front Microbiol. 2019;10:1416.
Mohamed-Romai-Noor NA, Sam SS, Teoh BT, Hamim ZR, AbuBakar S. Genomic and in vitro phenotypic comparisons of epidemic and non-epidemic Getah virus strains. Viruses. 2022;14:942.
Lu G, Chen R, Shao R, Dong N, Liu W, Li S, et al. Getah virus: an increasing threat in China. J Infect. 2020;80:350–71.
Li YY, Fu SH, Guo XF, Lei WW, Li XL, Song JD, et al. Identification of a newly isolated Getah virus in the China-Laos Border. China Biomed Environ Sci. 2017;30:210–4.
Shi N, Zhu X, Qiu X, Cao X, Jiang Z, Lu H, et al. Origin, genetic diversity, adaptive evolution and transmission dynamics of Getah virus. Transbound Emerg Dis. 2022;69:e1037–50.
Griffin DE. Alphaviruses. In: Knipe DM, Howley PM, editors. Fields virology. 6th ed. Philadelphia: Lippincott Williams & Wilkins; 2013. p. 651–86.
Sugiura T, Ando Y, Imagawa H, Kumanomido T, Fukunaga Y, Kamada M, et al. An epizootiological study of Getah virus among light horses in Japan in 1979. Bull Equine Res Inst. 1981;18:103–9.
Kawamura H, Yago K, Narita M, Imada T, Nishimori T, Haritani M. A fatal case in newborn piglets with Getah virus infection: pathogenicity of the isolate. Nihon Juigaku Zasshi. 1987;49:1003–7.
Yang T, Li R, Hu Y, Yang L, Zhao D, Du L, et al. An outbreak of Getah virus infection among pigs in China, 2017. Transbound Emerg Dis. 2018;65:632–7.
Zhao M, Yue C, Yang Z, Li Y, Zhang D, Zhang J, et al. Viral metagenomics unveiled extensive communications of viruses within giant pandas and their associated organisms in the same ecosystem. Sci Total Environ. 2022;820:153317.
Shi N, Li LX, Lu RG, Yan XJ, Liu H. Highly pathogenic swine Getah virus in blue foxes, eastern China, 2017. Emerg Infect Dis. 2019;25:1252–4.
Liu H, Zhang X, Li LX, Shi N, Sun XT, Liu Q, et al. First isolation and characterization of Getah virus from cattle in northeastern China. BMC Vet Res. 2019;15:320.
Kamada M, Ando Y, Fukunaga Y, Kumanomido T, Imagawa H, Wada R, et al. Equine Getah virus infection: isolation of the virus from racehorses during an enzootic in Japan. Am J Trop Med Hyg. 1980;29:984–8.
Sentsui H, Kono Y. An epidemic of Getah virus infection among racehorses: isolation of the virus. Res Vet Sci. 1980;29:157–61.
Takashima I, Hashimoto N. Getah virus in several species of mosquitoes. Trans R Soc Trop Med Hyg. 1985;79:546–50.
Tsuda Y, Kamezaki H. Mark-release-recapture study on movement of mosquitoes: individual marking method and short-term study of Aedes albopictus and Armigeres subalbatus in residential area on Ishigaki island. Japan Med Entomol Zool. 2014;65:61–6.
Yadav P, Gokhale MD, Barde PV, Singh DK, Mishra AC, Mourya DT. Experimental transmission of Chikungunya virus by Anopheles stephensi mosquitoes. Acta Virol. 2003;47:45–7.
Ishtiaq F, Swain S, Kumar SS. Anopheles stephensi (Asian Malaria Mosquito). Trends Parasitol. 2021;37:571–2.
World Health Organization. A global brief on vector-borne diseases. 2014. https://apps.who.int/iris/handle/10665/111008. Accessed 24 Dec 2022.
Kobayashi D, Isawa H, Ejiri H, Sasaki T, Sunahara T, Futami K, et al. Complete genome sequencing and phylogenetic analysis of a Getah Virus Strain (Genus Alphavirus, Family Togaviridae) isolated from Culex tritaeniorhynchus mosquitoes in Nagasaki, Japan in 2012. Vector Borne Zoonotic Dis. 2016;16:769–76.
Hotta S. Dengue vector mosquitoes in Japan: the role of Aedes albopictus and Aedes aegypti in the 1942–1944 dengue epidemics of Japanese Main Islands. Med Entomol Zool. 1998;49:267–74.
Amoa-Bosompem M, Kobayashi D, Itokawa K, Faizah AN, Kuwata R, Dadzie S, et al. Establishment and characterization of a cell line from Ghanaian Aedes aegypti (Diptera: Culicidae) focusing on Aedes-borne flavivirus susceptibility. In Vitro Cell Dev Biol Anim. 2020;56:792–8.
Miller JR, Koren S, Dilley KA, Puri V, Brown DM, Harkins DM, et al. Analysis of the Aedes albopictus C6/36 genome provides insight into cell line utility for viral propagation. Gigascience. 2018;7:1–13.
Walker T, Jeffries CL, Mansfield KL, Johnson N. Mosquito cell lines: history, isolation, availability and application to assess the threat of arboviral transmission in the United Kingdom. Parasit Vectors. 2014;7:382.
Vasilakis N, Deardorff ER, Kenney JL, Rossi SL, Hanley KA, Weaver SC. Mosquitoes put the brake on arbovirus evolution: experimental evolution reveals slower mutation accumulation in mosquito than vertebrate cells. PLoS pathog. 2009;5:e1000467.
Kimura T, Ueba N. Some biological and serological properties of large and small plaque variants of Getah virus. Arch Virol. 1978;57:221–9.
Shibata I, Hatano Y, Nishimura M, Suzuki G, Inaba Y. Isolation of Getah virus from dead fetuses extracted from a naturally infected sow in Japan. Vet Microbiol. 1991;27:385–91.
Igarashi A, Sasao F, Fukai K, Buei K, Ueda N, Yoshida M. Mutants of Getah and Japanese encephalitis viruses isolated from field-caught Culex tritaeniorhynchus using Aedes albopictus clone C6/36 cells. Ann Inst Pasteur Virol. 1981;132:235–45.
Hoshino K, Isawa H, Tsuda Y, Sawabe K, Kobayashi M. Isolation and characterization of a new insect flavivirus from Aedes albopictus and Aedes flavopictus mosquitoes in Japan. Virology. 2009;391:119–29.
Kuwata R, Hoshino K, Isawa H, Tsuda Y, Tajima S, Sasaki T, et al. Establishment and characterization of a cell line from the mosquito Culex tritaeniorhynchus (Diptera: Culicidae). I In Vitro Cell Dev Biol Anim. 2012;48:369–76.
Hoshino K, Isawa H, Kuwata R, Tajima S, Takasaki T, Iwabuchi K, et al. Establishment and characterization of two new cell lines from the mosquito Armigeres subalbatus (Coquillett)(Diptera: Culicidae). In Vitro Cell Dev Biol Anim. 2015;51:672–9.
Schneider I. Establishment of three diploid cell lines of Anopheles stephensi (Diptera: Culicidae). J Cell Biol. 1969;42:603–6.
Igarashi A. Isolation of a Singh’s Aedes albopictus cell clone sensitive to Dengue and Chikungunya viruses. J Gen Virol. 1978;40:531–44.
Ejiri H, Lim CK, Isawa H, Fujita R, Murota K, Sato T, et al. Characterization of a novel thogotovirus isolated from Amblyomma testudinarium ticks in Ehime, Japan: a significant phylogenetic relationship to Bourbon virus. Virus Res. 2018;249:57–65.
Amoa-Bosompem M, Kobayashi D, Itokawa K, Murota K, Faizah AN, Azerigyik FA, et al. Determining vector competence of Aedes aegypti from Ghana in transmitting dengue virus serotypes 1 and 2. Parasit Vectors. 2021;14:228.
Faizah AN, Kobayashi D, Amoa-Bosompem M, Higa Y, Tsuda Y, Itokawa K, et al. Evaluating the competence of the primary vector, Culex tritaeniorhynchus, and the invasive mosquito species, Aedes japonicus japonicus, in transmitting three Japanese encephalitis virus genotypes. PLoS Negl Trop Dis. 2020;14:e0008986.
R Development Core Team. R: A language and environment for statistical computing. Vienna: R Foundation for Statistical Computing. 2009. http://www.R-project.org. Accessed 17 Nov 2022.
Clem RJ. Arboviruses and apoptosis: the role of cell death in determining vector competence. J Gen Virol. 2016;97:1033–6.
Hardy JL, Houk EJ, Kramer LD, Reeves WC. Intrinsic factors affecting vector competence of mosquitoes for arboviruses. Annu Rev Entomol. 1983;28:229–62.
Hay S, Kannourakis G. A time to kill: viral manipulation of the cell death program. J Gen Virol. 2002;83:1547–64.
Richard A, Tulasne D. Caspase cleavage of viral proteins, another way for viruses to make the best of apoptosis. Cell Death Dis. 2012;3:e277.
Brackney DE, Scott JC, Sagawa F, Woodward JE, Miller NA, Schilkey FD, et al. C6/36 Aedes albopictus cells have a dysfunctional antiviral RNA interference response. PLoS Negl Trop Dis. 2010;4:e856.
Li YG, Siripanyaphinyo U, Tumkosit U, Noranate N, A-nuegoonpipat A, Tao R, et al. Chikungunya virus induces a more moderate cytopathic effect in mosquito cells than in mammalian cells. Intervirology. 2013;56:6–12.
White LA. Susceptibility of Aedes albopictus C6/36 cells to viral infection. J Clin Microbiol. 1987;25:1221–4.
Takashima I, Hashimoto N, Arikawa J, Matsumoto K. Getah virus in Aedes vexans nipponii and Culex tritaeniorhynchus: vector susceptibility and ability to transmit. Arch Virol. 1983;76:299–305.
Turell MJ, Mores CN, Dohm DJ, Lee WJ, Kim HC, Klein TA. Laboratory transmission of Japanese encephalitis, West Nile, and Getah viruses by mosquitoes (Diptera: Culicidae) collected near Camp Greaves, Gyeonggi Province, Republic of Korea, 2003. J Med Entomol. 2006;43:1076–81.
Russell RC. The mosquito fauna of Conjola State Forest on the south coast of New South Wales; part 4. The epidemiological implications for arbovirus transmission. Gen Appl Entomol. 1988;20:63–8.
Pennington NE, Phelps CA. Identification of the host range of Culex tritaeniorhynchus mosquitoes on Okinawa. Ryukyu Islands J Med Entomol. 1968;5:483–7.
Kawai S. Studies on the follicular development and feeding activity of the females of Culex tritaeniorhynchus with special reference to those in autumn. Trop Med. 1969;11:145–69.
Mims CA, Day MF, Marshall ID. Cytopathic effect of Semliki Forest virus in the mosquito Aedes aegypti. Am J Trop Med Hyg. 1966;15:775–84.
Kelly EM, Moon DC, Bowers DF. Apoptosis in mosquito salivary glands: Sindbis virus-associated and tissue homeostasis. J Gen Virol. 2012;93:2419–24.
Bowers DF, Coleman CG, Brown DT. Sindbis virus-associated pathology in Aedes albopictus (Diptera: Culicidae). J Med Entomol. 2003;40:698–705.
Girard YA, Klingler KA, Higgs S. West Nile virus dissemination and tissue tropisms in orally infected Culex pipiens quinquefasciatus. Vector Borne Zoonotic Dis. 2004;4:109–22.
Sawabe K, Imanishi-Kobayashi N, Maekawa Y, Higa Y, Kim KS, Hoshino K, et al. Updated distribution of anopheline mosquitoes in Hokkaido, Japan, and the first evidence of Anopheles belenrae in Japan. Parasit Vectors. 2021;14:494.
The authors wish to thank the members and staff of the Department of Parasitology and Tropical Medicine, Tokyo Medical and Dental University, the National Institute of Infectious Diseases for providing the platform to perform the study and offering constructive criticisms.
This work was supported by grants-in-aid for the Research Program on Emerging and Re-emerging Infectious Diseases from Japan Agency for Medical Research and development (AMED) Grant Numbers JP19fk0108035, JP20fk0108067, JP21fk0108123, and JP21fk0108613, and JSPS KAKENHI Grant Number JP18H02856.
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Additional file 1: Figure S1.
a Plot showing the TaqMan™ Fast Virus 1-Step Master Mix qRT-PCR output for 1:10 serial dilutions of the reference GETV RNA. GETV one-step proliferation curves were calculated between 1.0 × 1010 and 1.0 × 101 copies/µl. b A standard curve for GETV RNA was generated using 1:100 serial dilutions. The RNA dilution titers ranged from 1 × 1010 to 1 × 101. The equation derived from the quantitative real-time PCR assay was y = – 0.284x + 11.876, with R2 = 0.9997 and efficiency = 98.27. The Cq value was plotted on the y-axis, and the viral titers corresponding to the template RNA were plotted on the x-axis as log values.
Additional file 2: Figure S2.
Cell culture characterization of GETV infection and the morphological development of mosquito cell lines via microscopy analysis. Panels a-e represent the proliferation of uninfected Ae. albopictus-derived C6/36 and mock-infected C6/36 cells at each time point in hours (hpi). Panels f-j represent the proliferation of GETV-infected C6/36 cells at each time point after GETV infection. Panels k–o represent the proliferation of Cx. tritaeniorhynchus-derived NIID-CTR and mock-infected NIID-CTR cells at each time point. Panels m-q represent the proliferation of NIID-CTR cells at each time point post-GETV infection. Panels r-v represent the proliferation of uninfected Ar. subalbatus-derived Ar-3 and mock-infected Ar-3 cells at each time point. Panels w-aa represent the proliferation of Ar-3 cells at each time point after GETV infection. Panels bb-ff represent the proliferation of uninfected An. stephensi-derived MSQ43 and mock-infected MSQ43 cells at each time point. Panels gg-kk represent the proliferation of MSQ43 cells at each time point after GETV infection. hpi, Hours post-infection.
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Azerigyik, F.A., Faizah, A.N., Kobayashi, D. et al. Evaluating the mosquito host range of Getah virus and the vector competence of selected medically important mosquitoes in Getah virus transmission. Parasites Vectors 16, 99 (2023). https://doi.org/10.1186/s13071-023-05713-4
- Getah virus
- Culex tritaeniorhynchus
- Vector competence