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European Aedes albopictus and Culex pipiens Are Competent Vectors for Japanese Encephalitis Virus

European Aedes albopictus and Culex pipiens Are Competent Vectors for Japanese Encephalitis Virus

  • Mélissanne de Wispelaere, 
  • Philippe Desprès, 
  • Valérie Choumet
PLOS
x

Abstract

Background

Japanese encephalitis virus (JEV) is the causative agent of Japanese encephalitis, the leading cause of viral encephalitis in Asia. JEV transmission cycle involves mosquitoes and vertebrate hosts. The detection of JEV RNA in a pool of Culex pipiens caught in 2010 in Italy raised the concern of a putative emergence of the virus in Europe. We aimed to study the vector competence of European mosquito populations, such as Cx. pipiens and Aedes albopictus for JEV genotypes 3 and 5.

Findings

After oral feeding on an infectious blood meal, mosquitoes were dissected at various times post-virus exposure. We found that the peak for JEV infection and transmission was between 11 and 13 days post-virus exposure. We observed a faster dissemination of both JEV genotypes in Ae. albopictus mosquitoes, when compared with Cx. pipiens mosquitoes. We also dissected salivary glands and collected saliva from infected mosquitoes and showed that Ae. albopictus mosquitoes transmitted JEV earlier than Cx. pipiens. The virus collected from Ae. albopictus and Cx. pipiens saliva was competent at causing pathogenesis in a mouse model for JEV infection. Using this model, we found that mosquito saliva or salivary glands did not enhance the severity of the disease.

Conclusions

In this study, we demonstrated that European populations of Ae. albopictus and Cx. pipiens were efficient vectors for JEV transmission. Susceptible vertebrate species that develop high viremia are an obligatory part of the JEV transmission cycle. This study highlights the need to investigate the susceptibility of potential JEV reservoir hosts in Europe, notably amongst swine populations and local water birds.

Author Summary

Japanese encephalitis virus (JEV) is the leading cause of viral encephalitis in Asia. JEV is maintained in a cycle involving mosquitoes and vertebrate hosts, mainly pigs and wading birds. Humans can be infected when bitten by an infected mosquito. Culex tritaeniorhynchus is the main vector of the disease in tropical and subtropical areas. The recent detection of JEV in birds and mosquitoes collected in Northern Italy has led us to evaluate the putative emergence of this arboviral disease in Europe. For this purpose, we have tested the competence of European populations of Cx. pipiens and Aedes albopictus to transmit this virus in a laboratory setting. We showed that these local mosquitoes could be infected and were capable of transmitting a pathogenic virus to mice. It is thus urgent to evaluate the risks of JEV emergence in European regions displaying a favorable environment for mosquito vectors, susceptible pigs and wading birds.

Introduction

Japanese encephalitis is one of the major viral encephalitides in Asia, with an estimated 68,000 human cases per year [1]. Up to 30% of the symptomatic cases are fatal, and long-term neurologic sequelae can occur in 30 to 50% of survivors [2]. Japanese encephalitis virus (JEV) is the causative agent of Japanese encephalitis, and is transmitted through the bite of an infected mosquito. JEV is a member of the Flavivirus genus in the Flaviviridae family and has a positive-sense RNA genome. The viral polyprotein is processed into 10 proteins: three structural proteins and seven nonstructural proteins. JEV strains can be differentiated into five genotypes (1 to 5) based on phylogenetic studies of the viral envelope protein sequences. Until recently, most of the strains of JEV at the origin of major epidemics in the South, East and Southeast Asia regions belonged to genotype 3 [3, 4]. Recently a shift in prevalence from JEV genotype 3 to 1 has been observed in several Asian countries [57]. JEV genotype 5 was first isolated in Malaysia in 1952, and is genetically and serologically distinct from other genotypes [810]. No other JEV genotype 5 strain had been identified until its recent isolation from Culex spp. mosquito pools in China in 2009 [11] and in South Korea in 2010 and 2012 [12, 13].

Most of the vectors for JEV belong to the Culicinae subfamily in the Culicidae family. In most Asian countries, the main vector is Culex tritaeniorhynchus [7, 1418], while Cx. annulirostris was identified as the main vector for JEV transmission in Australia [19, 20]. Several secondary vectors are known to efficiently transmit JEV: Cx. annulirostris, Cx. annulus, Cx. fuscocephala, Cx. gelidus, Cx. sitiens or Cx. vishnui. The fact that JEV can be detected in field-caught mosquitoes belonging to numerous species, such as Cx. pipiens [12, 17, 21], Aedes albopictus [7, 22], or Anopheles species [7, 23], poses the question if those mosquito species could also act as secondary vectors for JEV.

The JEV enzootic cycle involves mosquitoes and amplifying vertebrate hosts, such as water birds and domestic swine [24]. Humans are considered as dead-end hosts, while they can be infected by JEV, they do not develop high levels of blood viremia, and thus cannot infect mosquitoes [25].

A fragment of JEV genome was detected in a pool of Cx. pipiens and in birds caught in 2000 and 2010 in Northern Italy [21, 26] raising the threat of a putative emergence of the virus in Europe [27]. Recent studies have shown that Ae. detritus from England and Ae. japonicus japonicus from Germany were competent to transmit JEV [28, 29]. These observations emphasize on the need to study the vector competence of European mosquito populations for JEV. Ae. albopictus is currently expanding its range, predominantly in temperate areas in North America and Europe, and this invasion raises a public health threat for pathogens transmitted by this vector, such as Zika and dengue viruses. Cx. pipiens is the most widely distributed species of mosquito in the world, and is typically found in temperate regions. Cx. pipiens complex mosquitoes play important roles in the transmission of several medically relevant pathogens such as West Nile virus (WNV), Saint Louis encephalitis virus, and filarial worms [3032].

In the present study, we evaluated the competence of Ae. albopictus and Cx. pipiens populations collected in the South of France for two representative strains of JEV, belonging to distinct genotypes. We found that both viruses could infect and disseminate to high efficiency in either vector and could be readily transmitted. We additionally evaluated the influence of mosquito salivary factors on viral pathogenesis and showed that they had no impact on the development of Japanese encephalitis in a mouse model for the disease. Overall, these findings highlight the need for investigation of the other factors that could contribute to JEV emergence in Europe.

Methods

Ethics statement

The protocols and subsequent experiments were ethically approved by the Ethic Committee for Control of Experiments on Animals (CETEA) at the Institut Pasteur and declared to the French Ministère de l’Enseignement Supérieur et de la Recherche (n° 000762.1) in accordance with European regulations. Experiments were conducted following the guidelines of the Office Laboratory of Animal Care at the Institut Pasteur. Euthanasia was performed by CO2 asphyxiation, followed by cervical dislocation. Anesthesia was performed by intraperitoneal injection of a mixture of Xylazine (Rompun, 5 to 10 mg/kg) and Kétamine (Imalgène, 80 to 100 mg/kg).

Mosquito rearing

Cx. pipiens form pipiens and Ae. albopictus mosquito colonies were established in the laboratory using mosquitoes collected in Montpellier and Nice, in 2010 and 2011, respectively. Eggs of each mosquito colony were hatched in tap water. Larvae were reared in plastic trays containing tap water supplemented with brewer’s yeast tablets and cat food. Adults were maintained at 27°C, 80% relative humidity with a 12 h:12 h light: dark cycle and were given continuous access to 10% sucrose solution.

Cells

Mosquito Ae. albopictus C6/36 cells were maintained at 28°C in Leibovitz medium (L15) supplemented with 10% heat-inactivated fetal bovine serum (FBS). Baby hamster kidney-derived BHK-21 (purchased from ATCC), chicken fibroblast-derived DF-1 (obtained from Nadia Naffakh), and human kidney-derived HEK293T cells (purchased from ATCC) were maintained at 37°C in DMEM supplemented with 10% FBS.

Antibodies

Mouse hybridomas producing the monoclonal antibody 4G2 anti-Flavivirus E were purchased from ATCC and a highly purified antibody preparation was produced by RD Biotech. The anti-mosquito saliva antibody was produced in house in rabbits exposed to mosquito bites. Horseradish peroxidase (HRP)-conjugated goat anti-mouse and anti-rabbit IgG antibodies were obtained from Bio-Rad Laboratories. Alexa Fluor 488-conjugated goat anti-mouse IgG antibody was obtained from Jackson ImmunoResearch.

Production of recombinant JEV

A molecular cDNA clone of JEV genotype 3 strain RP-9 was kindly provided by Yi-Lin Ling and was modified as described previously [33]. A molecular cDNA clone of JEV genotype 5 strain XZ0934 was described previously [33].

To produce infectious virus, the molecular clones were transfected into HEK293T cells using Lipofectamine 2000 (ThermoFischer Scientific). At 3 days post-transfection, viral supernatants were collected and used to infect DF-1 cells in order to grow final virus stocks for experiments.

Virus infections

For infections, C6/36 cells were seeded in 24-well tissue culture plates in L15, supplemented with 2% FBS. Aliquots of virus were diluted in 200 μl of medium and added to the cells. Plates were incubated for 1 h at 28°C. Unadsorbed virus was removed by two washes with Dulbecco's phosphate-buffered saline (DPBS) and then 1 ml of L15 supplemented with 2% FBS was added to the cells, followed by incubation at 28°C until collection.

Focus forming assay (FFA)

BHK-21 cells were seeded in 24-well plates. Tenfold dilutions of virus samples were prepared in duplicate in DMEM and 200 μl of each dilution was added to the cells. The plates were incubated for 1 h at 37°C. Unadsorbed virus was removed, after which 1 ml of DMEM supplemented with antibiotics and antifungals, 1.6% carboxymethyl cellulose (CMC), 10 mM HEPES buffer, 72 mM sodium bicarbonate, and 2% FBS was added to each well, followed by incubation at 37°C for 32 h. The CMC overlay was aspirated, and the cells were washed with PBS and fixed with 4% paraformaldehyde for 15 min, followed by permeabilization with 0.1% Triton-X100 for 5 min. After fixation, the cells were washed with PBS and incubated for 1 h at room temperature with anti-E antibody (4G2), followed by incubation with HRP-conjugated anti-mouse IgG antibody. The assays were developed with the Vector VIP peroxidase substrate kit (Vector Laboratories) according to the manufacturer’s instructions. The viral titers were expressed as focus forming units (FFU)/ml.

Oral infection of mosquitoes and dissections

Seven day-old female mosquitoes were deprived of sucrose 24 h prior to the infectious blood meal. They were then allowed to feed for 2 h on blood-soaked cotton pledgets in the dark at 28°C. The infectious blood meal was comprised of washed rabbit erythrocytes (obtained from animals housed at the Institut Pasteur animal facility), viral suspension, and ATP (as a phagostimulant) at a final concentration of 5 μM. The virus titer in the blood meal was adjusted to 8 x 106 FFU/ml. Blood-fed females were sorted and transferred into cardboard containers covered with mosquito nets. After exposure, engorged mosquitoes were maintained at 26°C, 80% relative humidity, with a 10 h: 10 h light: dark cycle with simulation of dawn and sunset during 2 h. Mosquitoes were dissected at various time points after oral exposure. For titrations, the mosquitoes or individual organs were collected in a tube containing 0.5 mm glass beads and 300 μl of DMEM supplemented with 2% FBS. The organs were ground for 30 sec at maximum speed, using a Minilystissue homogeneizer (Bertin) and stored at -80°C until analysis. Experiments were reproduced twice with 5 to 10 mosquitoes collected at each time point for dissection.

Mosquito salivation

JEV exposed mosquitoes were anesthetized at 4°C, legs and wings were removed and the bodies were attached to a glass slide using double-sided tape. The proboscis was manually inserted into a 10 μl low binding pipette tip filled with 10 μl DMEM containing 2% FBS. The tip contents were collected 30 min later in a tube. Two μl were transferred to a tube containing 2 μl SDS sample buffer and analyzed by dot-blot to verify the presence of saliva. Four μl were analyzed by FFA to determine virus titer. Ten to 20 mosquitoes were analyzed for each time point (days 11, 12 and 13 post-virus exposure) and experiments were reproduced twice.

Salivary gland extracts preparation

Five days after emerging, mosquito females were blood-fed on mice previously anesthetized by intraperitoneal injection of a mixture of Xylazine (5 to 10 mg/kg) and Ketamine (80 to 100 mg/kg). Three weeks later, 100 salivary glands (SG) were dissected and placed in 100 μl 1X PBS. SG extracts were prepared by sonicating the SG (five times at 4 min each with a pulse ratio of 2 sec on / 2 sec off) and centrifuging the crude extract at 10,000 g for 15 min at 4°C. The supernatant was transferred to clean tubes and stored at −80°C. The inocula used in our experiments contained the equivalent to a pair of SG.

Western blotting

Protein lysates were prepared by cell lysis in radio-immunoprecipitation assay (RIPA) buffer (Bio Basic) containing protease inhibitors (Roche). Equal amounts of proteins were loaded on a NuPAGE Novex 4–12% Bis-Tris protein gel (ThermoFisher Scientific) and transferred to a polyvinylidene difluoride membrane (Bio-Rad) using the Trans-Blot Turbo Transfer System (Bio-Rad). After blocking the membrane for 1 h at room temperature in PBS-Tween (PBS-T) plus 5% milk, the blot was incubated overnight at 4°C with appropriate dilutions of the primary antibodies. The membrane was then washed in PBS-T and then incubated for 1 h at room temperature in the presence of HRP-conjugated secondary antibodies. After washes in PBS-T, the membrane was developed using Pierce ECL Western Blotting Substrate (ThermoFisher Scientific) and exposed to film.

Dot-blot on mosquito saliva

The saliva collected from each mosquito was blotted onto a nitrocellulose membrane. Two μl of DMEM containing 2% FBS and 1 μg of mosquito salivary gland extract were deposited on the membrane as negative and positive controls, respectively. The membranes were blocked for 1 h in PBS-T plus 5% milk and incubated overnight at 4°C with an anti-mosquito saliva antibody. The blots were then processed as indicated above for Western blotting.

Immunofluorescence analysis (IFA)

After dissection, midguts (MG) and salivary glands (SG) were placed on slides and the PBS removed. MG were fixed in acetone for 15 min. SG were fixed in 4% paraformaldehyde for 15 min. Both slides were dried and stored at 4°C until use. The MG and SG were then rehydrated in PBS for 15 min. The MG and the SG were incubated in Triton X100 (0.2%) for 2 h and 15 min, respectively. They were then washed with PBS and incubated for 30 min with PBS + 0.1% Tween 20 containing 1% BSA. The slides were drained and incubated overnight at 4°C with anti-flavivirus protein E 4G2 antibody diluted in PBS, then washed with PBS. The slides were next incubated for 1 h with a fluorophore conjugated antibody, and washed with PBS. After washing, a drop of ProLong Gold Antifade reagent with DAPI (ThermoFisher Scientific) was placed on each slide and a cover slide was added. All preparations were examined using a fluorescence microscope (Axioplan 2 Imaging, Zeiss).

Mice experiments

Three-week-old female BALB/c mice were housed under pathogen-free conditions at the Institut Pasteur animal facility. Groups of mice were anesthetized as described above, and were next intradermally inoculated with 50 FFU of JEV genotype 5 in absence or in presence of salivary gland extract or with JEV-infected saliva diluted in 100 μl of DPBS supplemented with 0.2% endotoxin-free serum albumin.

Statistical analysis

An unpaired t test was used to compare quantitative data, and a Log-rank (Mantel-Cox) test was used to compare survival data. GraphPad Prism was used for all statistical analysis.

Animal handling

Rabbit and mice were housed in Institut Pasteur animal facilities.

Results

Vector competence of European strains of mosquitoes for JEV

To assess the vector competence of European mosquitoes for JEV, we decided to use two molecular clones of viruses (RP-9 and XZ0934), which are representative of two currently circulating genotypes. The well-characterized genotype 3 strain, JEV RP-9, was isolated from Cx. tritaeniorhynchus mosquitoes in Taiwan in 1985 [34, 35], while the genotype 5 strain, JEV-XZ0934, was recently isolated from Cx. tritaeniorhynchus mosquitoes in China in 2009 [11]. For simplification, JEV-RP-9 and JEV-XZ0934 will be hereafter referred to as JEV g3 and JEV g5, respectively. Both viruses were produced by transfection of cDNA into mammalian cells, as previously described [33], followed by amplification of viral stocks in chicken fibroblasts DF-1 cells. Those viruses displayed comparable growth after infection of Ae. albopictus derived C6/36 cells (Fig 1, [33]).

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Fig 1. Kinetics of JEV g3 and g5 infection in vitro.

Ae. albopictus derived C6/36 cells were infected with JEV g3 or g5 at a MOI of 1. The infectious virus released to the supernatants at 24, 48 and 72 h post-infection was quantified by FFA in BHK-21 cells. The error bars represent the standard deviation between two independent experiments (in each experiment, titrations were done on duplicate experimental samples). FFU, focus forming units.

https://doi.org/10.1371/journal.pntd.0005294.g001

To evaluate the vector competence of European mosquito species for JEV, we exposed mosquitoes to either JEV g3 or JEV g5 by feeding on blood meals containing approximately 8 x 106 FFU of virus per ml. We note that the viremia in infected pigs or in birds can reach up to 107 PFU/ml, but is on average 104 PFU/ml [3641]. While we offered blood meals that contained relatively high levels of virus, it is generally accepted that a greater quantity of virus is needed to infect mosquitoes orally with artificial mixtures than with viremic hosts [42]. For each experiment, 3 blood-fed mosquitoes were harvested immediately post-virus exposure, and the ingested virus titers were evaluated by FFA. The amount of ingested infectious virus was comprised between 400 and 9,000 FFU per mosquito, with an average titer of 4,000 FFU.

Previous studies on vector competence of various species of mosquitoes for JEV have shown the peak for JEV infection and transmission occurs between 5 and 23 days after peroral infection [23, 29, 4348]. Our preliminary studies showed that, under our experimental conditions, the majority of Cx. pipiens and Ae. albopictus were infected from 10 to 15 days post-virus exposure. We chose to focus collection times around the peak of viral transmission and harvested samples at 7, 11, 12 and 13 days post-virus exposure. We note that the survival rate of exposed mosquitoes dropped considerably after 2 weeks of infection, and consequently did not analyze the levels of mosquito infection beyond this point.

First, we determined the infection rates in Ae. albopictus (Fig 2A) and Cx. pipiens (Fig 2B) mosquitoes by titrating the midguts harvested from mosquitoes. Next, we measured the levels of JEV infection in the heads of infected mosquitoes, and calculated infected dissemination rates (Fig 2C and 2D). We did not observe any statistically significant differences in infection rates amongst genotypes for each mosquito species or by time after the infectious blood meal. We did note that dissemination of JEV was faster in Ae. albopictus mosquitoes, when compared with Cx. pipiens mosquitoes. Notably, at 7 days post-virus exposure, we found that 57 to 90% of Ae. albopictus mosquitoes were systemically infected, whereas only 26 to 36% of Cx. pipiens were (Fig 2C and 2D). Last, we determined transmission rates through titration of saliva collected from blood-fed mosquitoes (Fig 2E and 2F). While this is a method widely used to determined transmission rates, we observed that salivation assays are highly dependent on salivation efficiency, and that the levels of virus in saliva can sometimes be below the detection limit of our titration assay. Keeping in mind that this determination of the virus transmission rates has limitations, we observed that both mosquito species transmitted JEV at rates ranging from 20 to 63% for Ae. albopictus, and from 12 to 41% for Cx. pipiens (Fig 2E and 2F).

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Fig 2. Vector competence of European strains of mosquitoes for two different JEV genotypes following feeding on infectious bloodmeals.

Infection rates in Ae. albopictus (A) or Cx. pipiens (B) mosquitoes exposed to either JEV g3 or JEV g5 by feeding on blood meals containing 8 x 106 FFU/ml of virus. The infection rates were determined after titration of midguts harvested from mosquitoes on days 7, 11, 12 and 13 post-virus exposure. The infected dissemination rates (C and D) were calculated by titration of the heads of infected mosquitoes. The transmission rates (E and F) were calculated by titration of the saliva collected from all blood-fed mosquitoes. The error bars represent the standard deviation between two independent experiments. The number of mosquitoes analyzed for each condition is indicated below each graph bar. An unpaired t test was employed to determine significant differences between JEV genotypes at each time point. No statistically significant differences were found (P≥0.08). n.d. not determined.

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Characterization of JEV infection in European strains of mosquitoes

Next, we analyzed the levels of JEV g3 and g5 accumulation in the different mosquito organs that had been harvested (Fig 3). We noted that JEV levels in the midguts slowly decreased between 7 and 13 days post-virus exposure, while viral levels in heads and salivary glands increased over time, which is consistent with patterns of viral dissemination in mosquitoes. We noted that at 7 days post-virus exposure, the rates of salivary glands infection ranged from 40 to 80% for Ae. albopictus, and from 5 to 9% for Cx. pipiens. Viral infection of salivary glands has been shown to correlate well with infection of saliva [43], and thus we hypothesize that Ae. albopictus mosquitoes were likely to transmit JEV at earlier times than Cx pipiens. Interestingly, in Ae. albopictus mosquitoes midguts, we observed a significant difference in the titers of JEV g5 when compared to JEV g3 titers (Fig 3A). Notably, it appeared that JEV g5 accumulated to higher levels than JEV g3 at 7 days post-virus exposure, and to lesser levels at later infection times (11 to 13 days post-virus exposure).

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Fig 3. Kinetics of JEV infection in European strains of Ae. albopictus and Cx. pipiens mosquitoes.

Ae. albopictus (A, B and C) or Cx. pipiens (D, E and F) mosquitoes were exposed to either JEV g3 or JEV g5 by feeding on blood meals containing 8 x 106 FFU/ml of virus. At 7, 11, 12 and 13 days post-virus exposure, the midguts (A and D), heads (B and E) and salivary glands (C and F) were harvested from individual mosquitoes and the levels of infectious virus in each organ was quantified by FFA in BHK-21 cells. The error bars represent the standard deviation amongst infected samples collected from two independent experiments. An unpaired t test was employed to determine significant differences between JEV genotypes at each time point (***, P < 0.001; **, 0.001 < P < 0.01; *, 0.01 < P < 0.05; only statistically significant differences are shown).

https://doi.org/10.1371/journal.pntd.0005294.g003

Additionally, we analyzed the distribution of JEV envelope protein in the organs of infected mosquitoes (Fig 4). First, we performed immuno-localization within organs harvested from Ae. albopictus mosquitoes at 14 days post-virus exposure, which corresponds to a peak in viral transmission (Fig 4A). While envelope protein staining within the midgut was relatively weak, there was a strong staining of numerous cells within both lobes of salivary glands. Samples collected at 11 days post-virus exposure were also analyzed by western blotting and showed good detection of the envelope protein in midguts and salivary glands (Fig 4B).

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Fig 4. Analysis of JEV infection in mosquitoes.

A. Visualization of JEV envelope protein in the midgut (left panel) and salivary glands (right panel) of Ae. albopictus mosquitoes infected with JEV g3 at 14 days post-feeding on an infectious blood meal. Samples obtained from non-infected mosquitoes were used as a control (n.i.). Scale bars: 500 μm for the midgut samples, 50 μm for the salivary glands samples. B. Detection of JEV envelope protein in lysates obtained from midguts (top) and salivary glands (bottom) harvested from mosquitoes at 11 days post-feeding on an infectious blood meal. Samples from non-infected mosquitoes are used as a control (n.i.). The expected size for JEV envelope protein is indicated with an arrow.

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Detection of JEV in infected European mosquito saliva

To evaluate the levels of virus secreted in mosquito saliva, we collected mosquitoes at 11, 12 and 13 days post-feeding on an infectious blood meal, and performed forced salivation. Since not all of the mosquitoes salivate when subjected to this assay, we also performed a survey of successful salivation. A fraction of the collected saliva was dotted on a membrane, and was next incubated with an antibody specific for mosquito saliva (Fig 5A). We noted that both mosquito species efficiently salivated under our experimental conditions, and that the levels of actual salivation were above 40% for either mosquitoes (Fig 5A). The collected saliva was then subjected to a standard infectivity assay to determine the levels of JEV transmitted in JEV-positive saliva at each time point (Fig 5B and 5C). We noted that for both mosquito species, higher levels of virus were secreted in saliva at later times post-virus exposure, which mirrored the increase in viral load in salivary glands (Fig 3C and 3F). The levels of infectious virus in saliva ranged between 2 and 200 FFU for JEV g3 (45 and 55 FFU in average for Ae. albopictus and Cx. pipiens, respectively), and between 2 and 196 FFU for JEV g5 (38 and 35 FFU in average for Ae. albopictus and Cx. pipiens, respectively).

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Fig 5. Analysis of salivas collected from European mosquitoes infected by different genotypes of JEV.

At 11, 12 and 13 days post-virus exposure, salivas were collected from mosquitoes via forced salivation in pipette tips. A. Individual salivation samples were analyzed in a dot-blot assay using an anti-saliva antibody, to determine the salivation efficiency for each mosquito species. The rates of salivation obtained from two independent salivation assays are given, and a representative dot blot assay is shown. B. and C. The levels of infectious virus in JEV-positive saliva were measured by FFA in BHK-21 cells.

https://doi.org/10.1371/journal.pntd.0005294.g005

European mosquito saliva or salivary glands do not enhance JEV pathogenesis in a mouse model for JEV disease

Next we assessed whether the virus transmitted by European mosquitoes was capable of developing a productive infection in mammalian hosts. To evaluate this, we used a previously characterized murine model for Japanese encephalitis, based on JEV g5 infection of 3-week-old BALB/c mice [33]. Three-week-old BALB/c mice were injected via intradermal route with JEV, as this mode of injection most resembles a mosquito bite. First, JEV-positive saliva samples collected from Ae. albopictus and Cx. pipiens mosquitoes (Fig 5) were used as an inocula (Fig 6A). Saliva containing various loads of virus was used, with a titer comprised between 7 and 98 FFU. A control group of mice were similarly injected with JEV grown from C6/36 cells, using a single dose of 50 FFU (Fig 6A). As expected, the animals rapidly exhibited limb paralysis and encephalitis. We did not observe any significant differences in survival rates amongst the different inocula (Fig 6A). The survival rate was between 33 and 40%, with a mean survival time of 11 to 12.5 days.

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Fig 6. Effect of mosquito saliva and salivary glands on JEV infection in a mouse model.

Groups of 3-week-old BALB/c mice were monitored for survival after intradermal injection with JEV g5 (n = 6 per group). A. Mice were injected with JEV-positive saliva collected from infected mosquitoes. The levels of virus in saliva were between 7 and 98 FFU (Ae. albopictus: 9, 15, 22, 28, 60 and 70 FFU; Cx. pipiens: 7, 16, 24, 30, 51 and 98 FFU). Control mice were injected with 50 FFU of virus grown in C6/36 cells (C6/36 supernatants). B. Mice were injected with 50 FFU of virus, in presence or absence of one pair of salivary glands (SGP) harvested from either Ae. albopictus or Cx. pipiens mosquitoes. A Log-rank (Mantel-Cox) test was employed to determine significant differences between inocula. No statistically significant differences were found (P≥0.6).

https://doi.org/10.1371/journal.pntd.0005294.g006

The detection of JEV-specific antibodies showed that all surviving mice had been exposed to the virus (S1 Fig).

Since it was shown that mosquitoes can inject salivary components that influence the outcome of viral infection [4951], we next evaluated the impact of European mosquito salivary glands on JEV pathogenesis in a murine model. As described above, we used the intradermal route to inject 50 FFU of JEV g5 to 3-week-old BALB/c mice (Fig 6B). For two groups of mice, the inoculum was mixed with salivary glands extracts obtained from Ae. albopictus or Cx. pipiens mosquitoes. In accordance with what was previously observed after injection of saliva collected from infected mosquitoes, we did not observe any significant difference in the development of JEV pathogenesis in presence of mosquito salivary glands (Fig 6B). Overall these experiments show that European mosquitoes are fully competent at transmitting infectious JEV, but that saliva does not facilitate the development of viral pathogenesis in a susceptible murine model.

Discussion

In recent years, the increase in locally acquired exotic arbovirus diseases in Europe can be linked to the presence of appropriate combinations of vectors and vertebrate hosts, which could ultimately lead to the establishment of these diseases in Europe [5254]. Since 2010, sporadic cases of locally acquired chikungunya and dengue fevers have been noted in Europe [55, 56]. The driving forces behind these events are viraemic travelers and the increasing presence of competent vector species, such as Ae. aegypti and Ae. albopictus, in temperate regions. Likewise, the circulation of WNV and Usutu virus–two Flaviviruses—was reported in 10 European countries [57]. Two studies in Italy reported the infection of local Cx. pipiens populations with both WNV and Usutu virus [58, 59] and there is an increase in WNV disease incidence in Europe [60]. While JEV RNA was recently detected in mosquitoes and birds in Northern Italy [21, 26], to date, human infections with JEV were only reported in travelers returning from endemic countries [6163].

Our study shows for the first time that European strains of Cx. pipiens and Ae. albopictus are both competent vectors to transmit two genotypes (3 and 5) of JEV. High levels of infection, dissemination and transmission rates were observed in both vectors for either genotypes after oral exposure of mosquitoes to a blood meal containing virus at 8 x 106 FFU/ml. In the present study, we did not evaluate vector competence for viral strains belonging to the genotype 1. Strains belonging to this genotype have displaced the prevalent genotype 3 in several countries in recent years [57]. Genotype 1 and 3 strains are genetically close when compared to the more distant genotype 5 strains [810]. Since we observed equivalent vector competence of European mosquitoes for genotypes 3 and 5, we hypothesize that those mosquitoes will also be competent at transmitting genotype 1 viruses.

Several mosquitoes from the Culex genus are established vectors for JEV. Cx. tritaeniorhynchus is the main vector in the enzootic cycle of JEV in tropical and subtropical regions of Asia. Interestingly, the vector competence of a Cx. pipiens molestus population from Taiwan was found to be similar to that of Cx. tritaeniorhynchus, when tested in laboratory conditions [46], which is in line with our observations. Other investigators reported that Cx. pipiens populations from other world regions (Cx. pipiens molestus from Uzbekistan, Cx. pipiens pallens from Korea, Cx. pipiens from the United States of America) were less susceptible to JEV and were not always capable of transmitting the virus [50, 64]. Of note, there has been some reports of isolation of JEV from field-caught mosquitoes along the years [12, 17, 21, 65], and all strains of JEV isolated from Cx. pipiens mosquitoes in Korea in 2012 belonged to the genotype 5 [12]. As strains belonging to the genotype 5 were only rarely isolated, one can wonder if the transmission cycles that are involved in the maintenance of those viruses involve mosquito and amplifying host species different from the established Cx. tritaeniorhynchus / swine model. Since the currently available vaccines do not confer full protection against JEV genotype 5 strains [66, 67], the risks of JEV g5 transmission to human populations must be carefully examined.

Similarly to Cx. pipiens, field-collected Ae. albopictus mosquitoes were occasionally found positive for JEV [22, 68]. Various transmission rates were observed in laboratory settings, from less than 17% for Australian populations [69] to 45% for Taiwanese populations [22]. In our experiments, European Ae. albopictus was also able to transmit different strains of JEV to high efficiency, which supports the hypothesis that European mosquito populations belonging to these two species have a better vector competence for JEV than populations isolated in other parts of the world.

Our results also showed that the extrinsic incubation period (i.e. the time between ingestion of the virus and the ability of the mosquito to become infectious) for JEV is shorter in Ae. albopictus than in Cx. pipiens. We have not performed a formal analysis of the relative life span of our mosquito populations after ingestion of an infectious blood meal. If we assume that both mosquito species have similar life spans, then this would imply that Ae. albopictus mosquitoes can transmit JEV for a longer period than the French population of Cx. pipiens and therefore might be a more efficient vector. Specifically, host biting preferences may have consequences on the emergence of the disease in Europe and its transmission dynamics. Arbovirus circulation is defined by many aspects including the population dynamics of the mosquito vector, the extrinsic incubation period, and the population densities of the vertebrate amplifying hosts, all of which are influenced by environmental factors. In the case of JEV, the classic Cx. tritaeniorhynchus–pig transmission cycle was observed in Japan, a region of high pig farming density, but other species and scenarios could be invoked in regions where pig farming is less abundant, or where Cx. tritaeniorhynchus is not found [70]. An example of this is the 1995 outbreak of Japanese encephalitis in Australia that involved the presence of domestic pigs and high populations of Cx. annulirostris [19, 20]. Ae. albopictus is considered to be an opportunistic feeder: it primarily feeds on mammalian hosts (humans, wild and domestic animals) but can also acquire blood from avian sources [71, 72]. Analysis of feeding patterns in temperate regions showed that populations of Ae. albopictus in the United States of America mainly fed on mammals and rarely on birds [73]. Cx. pipiens mosquitoes feed mostly on birds (83%) but also on mammals [74]. Interestingly, it was shown that 20% of Cx. pipiens emerging from diapause in temperate habitats fed on mammals [73]. Considering the natural cycle of JEV implying birds as reservoir and pigs as amplifying hosts, specificity in host preferences may have consequences on the possible emergence of the disease in Europe and its transmission dynamics. Favorable conditions for JEV emergence may be gathered in several places in Europe where pig breeding sites, bird sanctuaries and Ae. albopictus and/or Cx. pipiens mosquitoes coexist (Marquenterre parc, Baie de Somme, France; Camargue, Rhone delta, France; Danube delta, Roumania).

The last part of our study was to investigate the role of mosquito saliva in the transmission of JEV to mice. When insects take a blood meal, they trigger defensive responses from the vertebrate, such as hemostasis and various immune responses. The saliva proteins injected by the mosquito can counteract these defenses, through their angiogenic, anti-hemostatic, anti-inflammatory and immunomodulatory properties [75]. This complex interaction may significantly affect the evolution of the disease; notably co-injection of virus and saliva was shown to potentiate infection of the vertebrate host by arboviruses belonging to various families [4951, 76, 77]. While we did not observe any enhancement of Japanese encephalitis disease in mice, in presence of salivary gland extract or of saliva collected from either European vectors, further studies are needed to evaluate the impact of saliva on viral burden in different organs. Additionally, we cannot exclude the possibility that JEV pathogenesis might be enhanced by salivary factors of other mosquito species, or that saliva from the two species tested in the present study might enhance pathogenicity in other mammalian species.

Conclusion

In this study, we have clearly demonstrated that European populations of Ae. albopictus and Cx. pipiens were efficient vectors for JEV transmission. Conditions for a putative emergence of JEV in Europe are linked to the possibility for an enzootic cycle to take place in temperate areas. In order to complete the infection cycle, JEV must be transmitted to a susceptible vertebrate host, capable of producing sufficient viral titers for subsequent acquisition by the insect vector. It is therefore important to further investigate whether any European swine or water birds populations can be infected with JEV and produce sufficiently high viremias to infect mosquitoes that feed on them. Such knowledge is critical to assess the potential for JEV to establish local transmission cycles similar to the closely related WNV in Northern Italy.

Supporting Information

S1 Fig. Detection of JEV specific antibodies in inoculated mice.

Sera were collected from mice at 28 days post-inoculation, and anti-JEV IgGs were quantified by ELISA using recombinant proteins corresponding to the domain III of JEV g5 envelope protein, as described in [33]. The ELISA absorbance values were measured at 450 nm and the absorbance value obtained from sera of mice inoculated with DPBS is shown as a dashed line (A450 nm = 0.042). Each symbol represents an individual mouse.

https://doi.org/10.1371/journal.pntd.0005294.s001

(DOCX)

Acknowledgments

We gratefully acknowledge Elisabeth Ferquel for help with mosquito rearing, Nadia Naffakh for the gift of DF-1 cells, and Yi-Lin Ling for providing the JEV-RP-9 cDNA clone.

Author Contributions

  1. Conceptualization: MdW PD VC.
  2. Formal analysis: MdW.
  3. Funding acquisition: PD.
  4. Investigation: MdW VC.
  5. Methodology: MdW VC.
  6. Visualization: MdW.
  7. Writing – original draft: MdW VC.
  8. Writing – review & editing: MdW PD VC.

References

  1. 1. Campbell GL, Hills SL, Fischer M, Jacobson JA, Hoke CH, Hombach JM, et al. Estimated global incidence of Japanese encephalitis: a systematic review. Bull World Health Organ. 2011;89(10):766–74, 74A–74E. pmid:22084515
  2. 2. Fischer M, Hills S, Staples E, Johnson B, Yaich M, Solomon T, et al. Japanese encephalitis prevention and control: advances, challenges, and new initiatives,. In: W M H S, H JM, editors. Emerging infections. 8. Washington, DC: American Society for Microbiology; 2008. p. 93–124.
  3. 3. Schuh AJ, Ward MJ, Brown AJ, Barrett AD. Phylogeography of Japanese encephalitis virus: genotype is associated with climate. PLoS Negl Trop Dis. 2013;7(8):e2411. pmid:24009790
  4. 4. Schuh AJ, Guzman H, Tesh RB, Barrett AD. Genetic diversity of Japanese encephalitis virus isolates obtained from the Indonesian archipelago between 1974 and 1987. Vector Borne Zoonotic Dis. 2013;13(7):479–88. pmid:23590316
  5. 5. Gao X, Liu H, Wang H, Fu S, Guo Z, Liang G. Southernmost Asia is the source of Japanese encephalitis virus (genotype 1) diversity from which the viruses disperse and evolve throughout Asia. PLoS Negl Trop Dis. 2013;7(9):e2459. pmid:24069502
  6. 6. Pan XL, Liu H, Wang HY, Fu SH, Liu HZ, Zhang HL, et al. Emergence of genotype I of Japanese encephalitis virus as the dominant genotype in Asia. J Virol. 2011;85(19):9847–53. Epub 2011/06/24. pmid:21697481
  7. 7. Su CL, Yang CF, Teng HJ, Lu LC, Lin C, Tsai KH, et al. Molecular epidemiology of Japanese encephalitis virus in mosquitoes in Taiwan during 2005–2012. PLoS Negl Trop Dis. 2014;8(10):e3122. pmid:25275652
  8. 8. Hasegawa H, Yoshida M, Fujita S, Kobayashi Y. Comparison of structural proteins among antigenically different Japanese encephalitis virus strains. Vaccine. 1994;12(9):841–4. pmid:7975862
  9. 9. Hasegawa H, Yoshida M, Kobayashi Y, Fujita S. Antigenic analysis of Japanese encephalitis viruses in Asia by using monoclonal antibodies. Vaccine. 1995;13(17):1713–21. pmid:8719524
  10. 10. Mohammed MA, Galbraith SE, Radford AD, Dove W, Takasaki T, Kurane I, et al. Molecular phylogenetic and evolutionary analyses of Muar strain of Japanese encephalitis virus reveal it is the missing fifth genotype. Infect Genet Evol. 2011;11(5):855–62. pmid:21352956
  11. 11. Li MH, Fu SH, Chen WX, Wang HY, Guo YH, Liu QY, et al. Genotype V Japanese encephalitis virus is emerging. PLoS Negl Trop Dis. 2011;5(7):e1231. pmid:21750744
  12. 12. Kim H, Cha GW, Jeong YE, Lee WG, Chang KS, Roh JY, et al. Detection of Japanese encephalitis virus genotype V in Culex orientalis and Culex pipiens (Diptera: Culicidae) in Korea. PLoS One. 2015;10(2):e0116547. pmid:25658839
  13. 13. Takhampunya R, Kim HC, Tippayachai B, Kengluecha A, Klein TA, Lee WJ, et al. Emergence of Japanese encephalitis virus genotype V in the Republic of Korea. Virol J. 2011;8:449. Epub 2011/09/29. pmid:21943222
  14. 14. Gajanana A, Rajendran R, Samuel PP, Thenmozhi V, Tsai TF, Kimura-Kuroda J, et al. Japanese encephalitis in south Arcot district, Tamil Nadu, India: a three-year longitudinal study of vector abundance and infection frequency. J Med Entomol. 1997;34(6):651–9. pmid:9439119
  15. 15. Lindahl JF, Stahl K, Chirico J, Boqvist S, Thu HT, Magnusson U. Circulation of Japanese encephalitis virus in pigs and mosquito vectors within Can Tho city, Vietnam. PLoS Negl Trop Dis. 2013;7(4):e2153. pmid:23593520
  16. 16. Scherer WF, Buescher EL, Flemings MB, Noguchi A, Scanlon J. Ecologic studies of Japanese encephalitis virus in Japan. III. Mosquito factors. Zootropism and vertical flight of Culex tritaeniorhynchus with observations on variations in collections from animal-baited traps in different habitats. Am J Trop Med Hyg. 1959;8:665–77. pmid:14442650
  17. 17. Seo HJ, Kim HC, Klein TA, Ramey AM, Lee JH, Kyung SG, et al. Molecular detection and genotyping of Japanese encephalitis virus in mosquitoes during a 2010 outbreak in the Republic of Korea. PLoS One. 2013;8(2):e55165. pmid:23390520
  18. 18. Tao Z, Liu G, Wang M, Wang H, Lin X, Song L, et al. Molecular epidemiology of Japanese encephalitis virus in mosquitoes during an outbreak in China, 2013. Sci Rep. 2014;4:4908. pmid:24809635
  19. 19. Ritchie SA, Phillips D, Broom A, Mackenzie J, Poidinger M, van den Hurk A. Isolation of Japanese encephalitis virus from Culex annulirostris in Australia. Am J Trop Med Hyg. 1997;56(1):80–4. pmid:9063367
  20. 20. Van Den Hurk AF, Johansen CA, Zborowski P, Paru R, Foley PN, Beebe NW, et al. Mosquito host-feeding patterns and implications for Japanese encephalitis virus transmission in northern Australia and Papua New Guinea. Med Vet Entomol. 2003;17(4):403–11. pmid:14651654
  21. 21. Ravanini P, Huhtamo E, Ilaria V, Crobu MG, Nicosia AM, Servino L, et al. Japanese encephalitis virus RNA detected in Culex pipiens mosquitoes in Italy. Euro Surveill. 2012;17(28). Epub 2012/07/28.
  22. 22. Weng MH, Lien JC, Wang YM, Wu HL, Chin C. Susceptibility of three laboratory strains of Aedes albopictus (Diptera: Culicidae) to Japanese encephalitis virus from Taiwan. J Med Entomol. 1997;34(6):745–7. pmid:9439133
  23. 23. Banerjee K, Deshmukh PK, Ilkal MA, Dhanda V. Experimental transmission of Japanese encephalitis virus through Anopheles tessellatus and Culex fatigans mosquitoes. Indian J Med Res. 1977;65(6):746–52. pmid:203526
  24. 24. Buescher EL, Scherer WF, Rosenberg MZ, Gresser I, Hardy JL, Bullock HR. Ecologic studies of Japanese encephalitis virus in Japan. II. Mosquito infection. Am J Trop Med Hyg. 1959;8:651–64. Epub 1959/11/01. pmid:13805722
  25. 25. Weaver SC, Barrett AD. Transmission cycles, host range, evolution and emergence of arboviral disease. Nat Rev Microbiol. 2004;2(10):789–801. pmid:15378043
  26. 26. Platonov A, Rossi G, Karan L, Mironov K, Busani L, Rezza G. Does the Japanese encephalitis virus (JEV) represent a threat for human health in Europe? Detection of JEV RNA sequences in birds collected in Italy. Euro Surveill. 2012;17(32).
  27. 27. Zeller H. Is Japanese encephalitis emerging in Europe? Euro Surveill. 2012;17(32).
  28. 28. Huber K, Jansen S, Leggewie M, Badusche M, Schmidt-Chanasit J, Becker N, et al. Aedes japonicus japonicus (Diptera: Culicidae) from Germany have vector competence for Japan encephalitis virus but are refractory to infection with West Nile virus. Parasitol Res. 2014;113(9):3195–9. pmid:24948103
  29. 29. Mackenzie-Impoinvil L, Impoinvil DE, Galbraith SE, Dillon RJ, Ranson H, Johnson N, et al. Evaluation of a temperate climate mosquito, Ochlerotatus detritus (= Aedes detritus), as a potential vector of Japanese encephalitis virus. Med Vet Entomol. 2015;29(1):1–9. pmid:25087926
  30. 30. Reisen WK, Milby MM, Meyer RP. Population dynamics of adult Culex mosquitoes (Diptera: Culicidae) along the Kern River, Kern County, California, in 1990. J Med Entomol. 1992;29(3):531–43. pmid:1625303
  31. 31. Turell MJ, Morrill JC, Rossi CA, Gad AM, Cope SE, Clements TL, et al. Isolation of West Nile and Sindbis viruses from mosquitoes collected in the Nile Valley of Egypt during an outbreak of Rift Valley fever. J Med Entomol. 2002;39(1):248–50. pmid:11931267
  32. 32. Bogh C, Pedersen EM, Mukoko DA, Ouma JH. Permethrin-impregnated bednet effects on resting and feeding behaviour of lymphatic filariasis vector mosquitoes in Kenya. Med Vet Entomol. 1998;12(1):52–9. pmid:9513939
  33. 33. de Wispelaere M, Frenkiel MP, Despres P. A Japanese encephalitis virus genotype 5 molecular clone is highly neuropathogenic in a mouse model: impact of the structural protein region on virulence. J Virol. 2015;89(11):5862–75. pmid:25787283
  34. 34. Chen LK, Lin YL, Liao CL, Lin CG, Huang YL, Yeh CT, et al. Generation and characterization of organ-tropism mutants of Japanese encephalitis virus in vivo and in vitro. Virology. 1996;223(1):79–88. pmid:8806542
  35. 35. Liang JJ, Liao CL, Liao JT, Lee YL, Lin YL. A Japanese encephalitis virus vaccine candidate strain is attenuated by decreasing its interferon antagonistic ability. Vaccine. 2009;27(21):2746–54. pmid:19366580
  36. 36. Nemeth N, Bosco-Lauth A, Oesterle P, Kohler D, Bowen R. North American birds as potential amplifying hosts of Japanese encephalitis virus. Am J Trop Med Hyg. 2012;87(4):760–7. pmid:22927494
  37. 37. Cleton NB, Bosco-Lauth A, Page MJ, Bowen RA. Age-related susceptibility to Japanese encephalitis virus in domestic ducklings and chicks. Am J Trop Med Hyg. 2014;90(2):242–6. pmid:24394476
  38. 38. Imoto J, Ishikawa T, Yamanaka A, Konishi M, Murakami K, Shibahara T, et al. Needle-free jet injection of small doses of Japanese encephalitis DNA and inactivated vaccine mixture induces neutralizing antibodies in miniature pigs and protects against fetal death and mummification in pregnant sows. Vaccine. 2010;28(46):7373–80. pmid:20851083
  39. 39. Konishi E, Pincus S, Paoletti E, Laegreid WW, Shope RE, Mason PW. A highly attenuated host range-restricted vaccinia virus strain, NYVAC, encoding the prM, E, and NS1 genes of Japanese encephalitis virus prevents JEV viremia in swine. Virology. 1992;190(1):454–8. pmid:1326813
  40. 40. Ricklin ME, Garcia-Nicolas O, Brechbuhl D, Python S, Zumkehr B, Posthaus H, et al. Japanese encephalitis virus tropism in experimentally infected pigs. Vet Res. 2016;47:34. pmid:26911997
  41. 41. 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(5):1076–81. pmid:17017248
  42. 42. Rosen L, Roseboom LE, Gubler DJ, Lien JC, Chaniotis BN. Comparative susceptibility of mosquito species and strains to oral and parenteral infection with dengue and Japanese encephalitis viruses. Am J Trop Med Hyg. 1985;34(3):603–15. pmid:2860816
  43. 43. Takahashi M. The effects of environmental and physiological conditions of Culex tritaeniorhynchus on the pattern of transmission of Japanese encephalitis virus. J Med Entomol. 1976;13(3):275–84. pmid:1011230
  44. 44. Bhatt TR, Crabtree MB, Guirakhoo F, Monath TP, Miller BR. Growth characteristics of the chimeric Japanese encephalitis virus vaccine candidate, ChimeriVax-JE (YF/JE SA14—14—2), in Culex tritaeniorhynchus, Aedes albopictus, and Aedes aegypti mosquitoes. Am J Trop Med Hyg. 2000;62(4):480–4. Epub 2001/02/28. pmid:11220763
  45. 45. Muangman D, Edelman R, Sullivan MJ, Gould DJ. Experimental transmission of Japanese encephalitis virus by Culex fuscocephala. Am J Trop Med Hyg. 1972;21(4):482–6. pmid:4340450
  46. 46. Weng MH, Lien JC, Lin CC, Yao CW. Vector competence of Culex pipiens molestus (Diptera: Culicidae) from Taiwan for a sympatric strain of Japanese encephalitis virus. J Med Entomol. 2000;37(5):780–3. pmid:11004796
  47. 47. van den Hurk AF, Nisbet DJ, Hall RA, Kay BH, MacKenzie JS, Ritchie SA. Vector competence of Australian mosquitoes (Diptera: Culicidae) for Japanese encephalitis virus. J Med Entomol. 2003;40(1):82–90. Epub 2003/02/25. pmid:12597658
  48. 48. Reid M, Mackenzie D, Baron A, Lehmann N, Lowry K, Aaskov J, et al. Experimental infection of Culex annulirostris, Culex gelidus, and Aedes vigilax with a yellow fever/Japanese encephalitis virus vaccine chimera (ChimeriVax-JE). Am J Trop Med Hyg. 2006;75(4):659–63. Epub 2006/10/14. pmid:17038690
  49. 49. Le Coupanec A, Babin D, Fiette L, Jouvion G, Ave P, Misse D, et al. Aedes mosquito saliva modulates Rift Valley fever virus pathogenicity. PLoS Negl Trop Dis. 2013;7(6):e2237. pmid:23785528
  50. 50. Styer LM, Lim PY, Louie KL, Albright RG, Kramer LD, Bernard KA. Mosquito saliva causes enhancement of West Nile virus infection in mice. J Virol. 2011;85(4):1517–27. pmid:21147918
  51. 51. Cox J, Mota J, Sukupolvi-Petty S, Diamond MS, Rico-Hesse R. Mosquito bite delivery of dengue virus enhances immunogenicity and pathogenesis in humanized mice. J Virol. 2012;86(14):7637–49. pmid:22573866
  52. 52. Grandadam M, Caro V, Plumet S, Thiberge JM, Souares Y, Failloux AB, et al. Chikungunya virus, southeastern France. Emerg Infect Dis. 2011;17(5):910–3. pmid:21529410
  53. 53. Gould EA, Gallian P, De Lamballerie X, Charrel RN. First cases of autochthonous dengue fever and chikungunya fever in France: from bad dream to reality! Clin Microbiol Infect. 2010;16(12):1702–4. pmid:21040155
  54. 54. Higgs S, Vanlandingham DL. The potential for the establishment of new arbovirus transmission cycles in Europe. Trans R Soc Trop Med Hyg. 2015;109(9):543–4. pmid:26246250
  55. 55. Sam IC, Kummerer BM, Chan YF, Roques P, Drosten C, AbuBakar S. Updates on chikungunya epidemiology, clinical disease, and diagnostics. Vector Borne Zoonotic Dis. 2015;15(4):223–30. pmid:25897809
  56. 56. Rezza G. Dengue and chikungunya: long-distance spread and outbreaks in naive areas. Pathog Glob Health. 2014;108(8):349–55. pmid:25491436
  57. 57. Nikolay B. A review of West Nile and Usutu virus co-circulation in Europe: how much do transmission cycles overlap? Trans R Soc Trop Med Hyg. 2015;109(10):609–18. pmid:26286946
  58. 58. Calzolari M, Bonilauri P, Bellini R, Albieri A, Defilippo F, Maioli G, et al. Evidence of simultaneous circulation of West Nile and Usutu viruses in mosquitoes sampled in Emilia-Romagna region (Italy) in 2009. PLoS One. 2010;5(12):e14324. pmid:21179462
  59. 59. Tamba M, Bonilauri P, Bellini R, Calzolari M, Albieri A, Sambri V, et al. Detection of Usutu virus within a West Nile virus surveillance program in Northern Italy. Vector Borne Zoonotic Dis. 2011;11(5):551–7. pmid:20849275
  60. 60. Rizzoli A, Bolzoni L, Chadwick EA, Capelli G, Montarsi F, Grisenti M, et al. Understanding West Nile virus ecology in Europe: Culex pipiens host feeding preference in a hotspot of virus emergence. Parasit Vectors. 2015;8:213. pmid:25888754
  61. 61. Lagarde S, Lagier JC, Charrel R, Querat G, Vanhomwegen J, Despres P, et al. Japanese encephalitis in a French traveler to Nepal. J Neurovirol. 2014;20(1):99–102. pmid:24408307
  62. 62. Langevin S, Libman M, Drebot MA, Laverdiere M. A case of Japanese encephalitis virus infection acquired during a trip in Thailand. J Travel Med. 2012;19(2):127–9. pmid:22414040
  63. 63. Lehtinen VA, Huhtamo E, Siikamaki H, Vapalahti O. Japanese encephalitis in a Finnish traveler on a two-week holiday in Thailand. J Clin Virol. 2008;43(1):93–5. pmid:18556242
  64. 64. Turell MJ, Mores CN, Dohm DJ, Komilov N, Paragas J, Lee JS, et al. Laboratory transmission of Japanese encephalitis and West Nile viruses by molestus form of Culex pipiens (Diptera: Culicidae) collected in Uzbekistan in 2004. J Med Entomol. 2006;43(2):296–300. pmid:16619614
  65. 65. Carey DE, Myers RM. Japanese encephalitis studies in Vellore, South India. 3. Neutralizing activity of human survey sera. Indian J Med Res. 1968;56(9):1330–9. pmid:4302908
  66. 66. Cao L, Fu S, Gao X, Li M, Cui S, Li X, et al. Low protective efficacy of the current Japanese encephalitis vaccine against the emerging genotype 5 Japanese encephalitis virus. PLoS Negl Trop Dis. 2016;10(5):e0004686. pmid:27139722
  67. 67. Tajima S, Yagasaki K, Kotaki A, Tomikawa T, Nakayama E, Moi ML, et al. In vitro growth, pathogenicity and serological characteristics of the Japanese encephalitis virus genotype V Muar strain. J Gen Virol. 2015;96(9):2661–9. pmid:26048886
  68. 68. Su T, Cheng ML, Melgoza A, Thieme J. Laboratory and field evaluations of Mosquiron(R) 0.12CRD, a new formulation of Novaluron, against Culex mosquitoes. J Am Mosq Control Assoc. 2014;30(4):284–90. pmid:25843134
  69. 69. Nicholson J, Ritchie SA, van den Hurk AF. Aedes albopictus (Diptera: Culicidae) as a potential vector of endemic and exotic arboviruses in Australia. J Med Entomol. 2014;51(3):661–9. pmid:24897860
  70. 70. Lord JS, Gurley ES, Pulliam JR. Rethinking Japanese encephalitis virus transmission: a framework for mplicating host and vector species. PLoS Negl Trop Dis. 2015;9(12):e0004074. pmid:26657648
  71. 71. Eritja R, Escosa R, Lucientes J, Marques E, Roiz D, Ruiz S. Worldwide invasion of vector mosquitoes: present European distribution and challenges in Spain. Biological Invasions. 2005;7(1).
  72. 72. Turell MJ, Dohm DJ, Sardelis MR, Oguinn ML, Andreadis TG, Blow JA. An update on the potential of north American mosquitoes (Diptera: Culicidae) to transmit West Nile Virus. J Med Entomol. 2005;42(1):57–62. pmid:15691009
  73. 73. Faraji A, Gaugler R. Experimental host preference of diapause and non-diapause induced Culex pipiens pipiens (Diptera: Culicidae). Parasit Vectors. 2015;8:389. pmid:26205410
  74. 74. Hamer GL, Kitron UD, Goldberg TL, Brawn JD, Loss SR, Ruiz MO, et al. Host selection by Culex pipiens mosquitoes and West Nile virus amplification. Am J Trop Med Hyg. 2009;80(2):268–78. pmid:19190226
  75. 75. Gillespie RD, Mbow ML, Titus RG. The immunomodulatory factors of bloodfeeding arthropod saliva. Parasite Immunol. 2000;22(7):319–31. pmid:10886716
  76. 76. Edwards JF, Higgs S, Beaty BJ. Mosquito feeding-induced enhancement of Cache Valley virus (Bunyaviridae) infection in mice. J Med Entomol. 1998;35(3):261–5. pmid:9615544
  77. 77. Schneider BS, Higgs S. The enhancement of arbovirus transmission and disease by mosquito saliva is associated with modulation of the host immune response. Trans R Soc Trop Med Hyg. 2008;102(5):400–8. pmid:18342898