Skip to main content

A novel assay to isolate and quantify third-stage Dirofilaria immitis and Brugia malayi larvae emerging from individual Aedes aegypti



Mosquitoes transmit filarial nematodes to both human and animal hosts, with worldwide health and economic consequences. Transmission to a vertebrate host requires that ingested microfilariae develop into infective third-stage larvae capable of emerging from the mosquito proboscis onto the skin of the host during blood-feeding. Determining the number of microfilariae that successfully develop to infective third-stage larvae in the mosquito host is key to understanding parasite transmission potential and to developing new strategies to block these worms in their vector.


We developed a novel method to efficiently assess the number of infective third-stage filarial larvae that emerge from experimentally infected mosquitoes. Following infection, individual mosquitoes were placed in wells of a multi-well culture plate and warmed to 37 °C to stimulate parasite emergence. Aedes aegypti infected with Dirofilaria immitis were used to determine infection conditions and assay timing. The assay was also tested with Brugia malayi-infected Ae. aegypti.


Approximately 30% of Ae. aegypti infected with D. immitis and 50% of those infected with B. malayi produced emerging third-stage larvae. Once D. immitis third-stage larvae emerged at 13 days post infection, the proportion of mosquitoes producing them and the number produced per mosquito remained stable until at least day 21. The prevalence and intensity of emerging third-stage B. malayi were similar on days 12–14 post infection. Increased uptake of D. immitis microfilariae increased the fitness cost to the mosquito but did not increase the number of emerging third-stage larvae.


We provide a new assay with an associated set of infection conditions that will facilitate assessment of the filarial transmission potential of mosquito vectors and promote preparation of uniformly infectious third-stage larvae for functional assays. The ability to quantify infection outcome will facilitate analyses of molecular interactions between vectors and filariae, ultimately allowing for the establishment of novel methods to block disease transmission.


Arthropods serve as intermediate hosts and vectors of numerous human and animal infective filariae that contribute to a large disease burden worldwide. Indeed, mosquito-transmitted lymphatic filariasis, caused by Wuchereria bancrofti, Brugia malayi and B. timori, affects approximately 120 million people in 83 countries [1]. Mosquitoes are also responsible for transmission of animal infective filariae, the most studied being Dirofilaria immitis, the causative agent of canine heartworm disease. Although detailed global numbers are not available, there are an estimated 250,000–500,000 infected dogs in the USA, with some areas, such as the Mississippi River basin, reporting infection prevalence as high as 40% [2, 3]. Humans can also be incidentally infected by D. immitis, but they do not support the entire life cycle and typically present with only mild clinical signs [3].

Within the mosquito host, ingested microfilariae (mf) migrate from the midgut to specific tissues specific to the mosquito species. The filarial agents of lymphatic filariasis migrate to the indirect flight muscles in the thorax, whereas D. immitis migrates into the Malpighian tubules (MT) [4]. In these tissues, the parasites develop intracellularly, undergoing successive molts to form third-stage larvae (L3). Some L3 migrate to the proboscis where they are poised for transmission (Additional file 1: Movie 1). Infective L3 emerge most typically from the mosquito labellum but they can also emerge from the labial sheath during blood-feeding (Fig. 1) [5]. Larvae emerging from the mosquito are deposited onto the skin in a drop of hemolymph where they can enter the skin through the bite site [5]. The fate of the L3 that do not emerge is not known.

Fig. 1

Emergence of infective third-stage larvae (L3) from the tip of the mosquito proboscis. During blood-feeding, a subpopulation of L3 in the labial sheath of the proboscis emerge from the proboscis, alighting on the skin of the host in a drop of the mosquito hemolymph (eL3). It is estimated that only approximately 10% of the eL3 survive on the skin and penetrate into it [26]; the fate of the L3 that do not emerge during blood-feeding is not known. Emergence from the proboscis typically occurs at the labellum or distal portion of the labial sheath and can be triggered by sensation of a thermal cue (red gradient). Other cues may also play a role, such as chemical compounds released by the host (green gradient) or a sensation of mechanical forces caused by the deformation of the labial sheath (orange gradient), which slides backward as the fascicle is inserted into the host skin. Adapted from Bancroft [36]

Due to their importance to the disease cycle, much attention is focused on the transmission of infective L3. Different methods have been employed to assay L3 in mosquitoes. A common approach, especially for field isolates, is the detection by PCR of larvae in the head and other body parts of the mosquito following dissection [6,7,8]. Although this method is not established for all filariae, stage-specific PCR has been used for detection of infectious L3 in W. bancrofti infected mosquitoes [9]. PCR is sensitive and species specific and can be used on pools of mosquitoes in cases where infection prevalence is low. Another commonly used approach is to physically examine larvae in the labial sheath of the proboscis or in dissected tissues of the mosquito. This approach is particularly useful in a laboratory setting to determine the number of larvae at each developmental stage and to identify their tissue of residence. However, while each of these assays can reveal the number of L3 that have developed, specific assays to enumerate L3 capable of emerging (eL3) when the mosquito blood-feeds have not been previously described.

In addition to assessing the intensity of transmission in field populations, an ability to enumerate and collect L3 capable of emergence would greatly enhance functional assessment. Currently, studies of host immune responses to L3, as well as in vitro and in vivo drug efficacy studies, are typically carried out on L3 collected from infected mosquitoes gently disrupted with a mortar and pestle and then separated by filtration though a mesh [10,11,12]. However, it is unknown whether all L3 harvested by this method are mature and competent to infect the host. Furthermore, obtaining microfilaria for mosquito infections requires access to an infected animal or access to samples from another source, and although D. immitis microfilaria have been shown to be capable of cryopreservation [13], this method of storage is not commonly used. More typically, fresh samples are shipped, despite being infective, little is known about how short-term storage during shipping affects development to L3.

Blocking parasite development in the vector is a novel approach being considered for controlling disease transmission and requires a thorough understanding of the molecular interactions between parasites and their vector. The means to quantify the prevalence of mosquitoes with eL3 and determine the number of emerging L3 per mosquito would greatly facilitate this work. Here we present a new assay to quantify infectious eL3 that works with different vector and filarial species. We then use this assay to study the development and characteristics of D. immitis eL3 in mosquitoes. The detailed infection parameters and assay conditions presented here to quantify and produce maximum yields of eL3 could potentially facilitate both studies between filariae and their mosquito and vertebrate hosts.


Mosquito strains and culture

Aedes aegypti and Ae. albopictus strains were provided by the National Institutes of Health/National Institute of Allergy and Infectious Diseases (NIH/NIAID) Filariasis Research Reagent Resource Center (FR3) and the Malaria Research and Reference Reagent Resource Center (MR4) through distribution by the NIH/NIAID BEI Resources Repository. Aedes aegyptiS (Ae. aegypti, Strain Black Eye Liverpool, Eggs, FR3, NR-48921) is a Dirofilaria immitis- and Brugia malayi-susceptible strain, and Ae. aegyptiR (Ae. aegypti, Strain LVP-IB12, Eggs, MR4, MRA-735, contributed by David W. Severson) is a D. immitis- and B. malayi-refractory strain. Both strains were reared at 27 °C and 80% humidity under a 12/12-h photoperiod. Aedes albopictusNJ (Ae. albopictus Strain ATM-NJ95, Eggs, MR4, NR-48979) [14] was reared at 24 °C and 70% humidity under a 16/8-h (light/dark) photoperiod. Mosquitoes were housed in 30-cm3 cages (BugDorm, Taichung, Taiwan) at a density of approximately 1000 per cage. Larvae were maintained at a density of 1 larva/3 ml. Larvae were fed a suspension of liver powder in water (MP Biomedicals, Solon, OH, USA), and adults were maintained on 10% sucrose in water, which was changed daily. Heparinized sheep blood (Hemostat, Dixon, CA, USA) was provided using an artificial membrane feeder at 37 °C for egg production.

Mosquito infection with Dirofilaria immitis and Brugia malayi

The full protocol is described in greater detail by Povelones and McCrea [15]. Blood containing D. immitis microfilariae was obtained from an experimentally infected dog according to Institutional Animal Care and Use Committee-approved protocols and in accordance with the guidelines of the Institutional Animal Care and Use Committee of the University of Pennsylvania (IACUC, protocol 805059). The microfilarial load in this dog was approximately 50,000 mf/ml. Blood containing B. malayi microfilariae (B. malayi microfilariae in cat blood, live, FR3, NR-48887) was obtained from an experimentally infected cat containing with a microfilarial load of approximately 12,000 mf/ml (provided by the NIH/NIAID FR3 for distribution by BEI Resources, NIAID/NIH). In both cases, the blood was diluted with the appropriate volume of heparinized sheep blood to a concentration of 4000 mf/ml. The sample was warmed to 37 °C, and a 3.5-ml aliquot was placed in the indentation on the outside of the bottom of a 300-ml plastic baby bottle (Advent; Phillips, Amsterdam, the Netherlands) and covered with Parafilm. The inside of the bottle was filled with water at 37 °C. This assembly was placed with the membrane side down onto the top mesh of mosquito cages and the insects are allowed to feed for 15 min (Fig. 2a). Immediately following the feed, fully engorged blood-fed mosquitoes were separated using CO2 anesthesia and housed under standard insectary conditions as described above. Any partial or unfed mosquitoes were discarded.

Fig. 2

Assay for eL3. a Infection and assay protocol followed in this study. Mosquitoes are fed on blood containing Dirofilaria immitis microfilariae. Uptake is measured in a small group, and the remaining mosquitoes are maintained until an emergence assay is performed. Immediately following the emergence assay with whole mosquitoes, the Malpighian tubules are dissected and analyzed. The dissected head and carcass are individually placed into an emergence assay to assay L3 that failed to emerge from intact mosquitoes. Additional file 2: Figure S1 shows images of dissected mosquitoes and Malpighian tubules. b, c Mosquitoes are rinsed with 70% ethanol:30% water for wetting, rinsed with water (b) and then placed individually into wells of a 96-well plate (c). d Emerging eL3 from intact mosquitoes or L3 from dissected heads and carcasses at the bottom each well are scored by microscopy. Additional file 3: Movie 2 shows typical movement of eL3. e Larvae (white arrows) in live Malpighian tubules are scored by microscopy. Scale bar: 50 µm

Microfilarial uptake

Within 1 hour of blood-feeding, fed mosquitoes were anesthetized with CO2 at room temperature. The entire undamaged midgut was dissected in deionized water in a depression slide and immediately transferred to a standard microscope slide containing a 50-µl drop of deionized water. Damaged midguts leaking blood during dissection were not used. The epithelium of the gut was separated from the blood bolus and moved through the water to remove any residual blood before it was discarded. The blood was roughly dispersed using forceps and then pipetted up-and-down with a 20-µl pipette. Microfilaria in the entire drop were counted immediately without a coverslip.

Emergence assay for eL3 and other larval stages

The full protocol is described in greater detail by Povelones and McCrea [16], which is modified from a previously published method [17]. Briefly, eL3 were assayed by placing live mosquitoes in 70% ethanol in water for 1 min, following which they were rinsed twice in deionized water and then placed individually into wells of a 96-well plate containing 200 µl Dulbecco’s Modified Eagle’s Medium (DMEM) supplemented with l-glutamine, a high level of glucose and sodium pyruvate (Corning Mediatech, Manassas, VA, USA). At this point, the mosquitoes are still alive and can be observed moving in the buffer, but they cannot stand on the surface due to the wetting procedure. The plate was then placed in a 37 °C incubator with 5% CO2 for 60 min, and the number of eL3 were determined without removing the mosquitoes using an inverted microscope with a ×4 objective. In some experiments, after the eL3 emergence assay, mosquitoes were removed from the plate individually for assaying other larvae. First, the Malpighian tubules were dissected by removing the posterior two abdominal segments. The set of five Malpighian tubules was removed from the midgut and transferred to a microscope slide containing 15 µl phosphate buffered saline and covered with a 22-mm2 coverslip. The larvae were counted, and although different stages were present we did not categorize them (Additional file 4: Figure S2). The head was then separated from the body, and the dissected head and carcass fragment were placed separately into fresh wells of a 96-well plate prepared and incubated as described above. L3 were allowed to migrate out of the dissected tissue for at least 60 min and scored as described above. Only a portion of the mosquitoes, between 30 and 36 from each replicate, used for the eL3 emergence assay were processed in this manner due to processing time constraints.

Emergence assay time course and microfilaria concentration series

Groups of 432–565 mosquitoes were fed on blood containing D. immitis microfilariae at different concentrations and housed as described above. Mosquito mortality was monitored daily, as assessed by the fraction of the population that died each day. This was necessary since groups of 50 mosquitoes were removed for eL3 assays as described above. Since the emergence prevalence was very low on day 12, emergence assays were performed with only 25 mosquitoes per replicate saving more of the population for later days where there would be a higher eL3 prevalence. For the concentration-series experiments, a blood dilution containing 32,000 mf/ml was created and then subjected to twofold serial dilution to create feeding doses of 16,000, 8000 and 4000 mf/mL. At each concentration, five mosquitoes of each strain were used to measure uptake, as described above. For these experiments, mortality was monitored daily until day 17 when an assay for eL3 was performed on the remaining mosquitoes. Kaplan–Meier survival analysis was performed between adjacent doses within each mosquito strain and between the same doses across the mosquito strains.


Novel assay for filarial nematode L3 emerging from individual mosquitoes

In our assay, outlined in Fig. 2a, we infect mosquitoes using an artificial membrane feeder and then determine the number of microfilariae ingested immediately afterwards [15]. The microfilarial uptake represents the theoretical maximum number of parasites in the assay. To assay the L3 capable of emerging from the mosquitoes, we simulate the thermal cue that would be experienced by a mosquito landing on a mammalian vertebrate host by placing mosquitoes in buffer and warming the buffer to 37 °C [16]. Mosquitoes are placed individually into wells of a 96-well plate after the wetting procedure (Fig. 2b, c), and care is taken to minimize damage to the mosquito during transfer. Upon warming, competent L3 emerge from the mosquito and sink to the bottom of the well, where they can be counted (Fig. 2d; Additional file 3: Movie 2). eL3 collected by this method are capable of molting to the fourth larval stage in vitro [18] and are infectious to dogs [17], and we believe they represent the number of L3 that emerge onto the skin of the host. After the emergence assay, the mosquitoes are still viable and can move, but they cannot escape the buffer due to the wetting procedure. Notably, following the emergence assay, further analyses can be carried out to determine the number and location of larvae remaining within the mosquito. In our study, both dissected Malpighian tubules (Fig. 2e), and the head and remaining carcass were assayed separately, as described in the following section (Additional file 2: Figure S1).

Microfilariae robustly migrate into the Malpighian tubules but only a fraction develop to eL3

To determine the efficiency of eL3 development we infected D. immitis susceptible (Ae. aegyptiS) or refractory (Ae. aegyptiR) strains and performed an emergence assay 14 dpi. We found that Ae. aegyptiR released no eL3, despite having a median uptake of 12 mf/mosquito (Fig. 3a). This is consistent with previous observations that ingested microfilariae arrest their development soon after invading cells of the Malpighian tubules [19,20,21,22,23]. In the susceptible strain (Ae. aegyptiS), 81 of the 252 mosquitoes assayed (32%) had at least one eL3 when given a median uptake of 15 mf/mosquito (Fig. 3b). A portion of the susceptible mosquitoes used for the emergence assay were dissected, and a substantial number had L3 remaining in the dissected heads (26/102; 25%) and carcasses (48/102; 47%) (Fig. 3b). The majority of larvae assayed at 14 dpi were present in the Malpighian tubules, and nearly all of the dissected mosquitoes (93/96; 97%) had at least one larva present in the Malpighian tubules (Fig. 3b). In a few cases, Malpighian tubules were damaged during the dissection and excluded from this and subsequent analyses. Pooling all larvae present across all tissues revealed that the median total number of larvae per mosquito was eight. Therefore, at 14 dpi, 53% of the 15 ingested microfilariae could be accounted for as larvae in the mosquito (Fig. 3b). In the dissected Malpighian tubules, we found larvae in various stages of development, but we did not determine their stage (Additional file 4: Figure S2). We note, however, that larvae found in the Malpighian tubules, even the most stunted sausage forms, are viable, as we observed them to be capable of movement. Previous studies suggest that not all L3 emerge when infected mosquitoes blood-feed on an animal [5]. Since this previous observation was not quantitative, we analyzed the data from the emergence assay (Fig. 3b) to compare the number of eL3 to the total L3 (eL3 + L3 in dissected heads, and dissected carcasses). We did not include larvae found in the Malpighian tubules since we could not unambiguously characterize them as L3. We found that the number of eL3 was significantly lower than the total L3 (Fig. 3c). Therefore, we concluded that only a fraction of the larvae that develop to L3 emerge during our emergence assay, consistent with previous observations [5].

Fig. 3

A fraction of ingested microfilariae develops into eL3 in Aedes aegyptiS (a D. immitis- and Brugia malayi-susceptible strain). a Dots indicate the number of microfilariae present in the midgut of individual Ae. aegyptiR (a D. immitis- and B. malayi-resistant strain) immediately after feeding on infected blood (Uptake) and the number of eL3 assayed 14 days post infection (dpi). The black line indicates the median. b Dots indicate the number of microfilariae present in the midgut of individual Ae. aegyptiS immediately after feeding on infected blood (Uptake), the number of eL3 assayed 14 dpi (eL3), the number of L3 emerging from the dissected heads (Head) or carcass (Carcass) and the number present in the Malpighian tubules (MT). The Total is sum of all parasites of any stage found in any tissue or assay on 14 dpi. The red line indicates the median. c Dots are the number of eL3 from individual Ae. aegyptiS and all third-stage larvae assayed (Total; sum of eL3, Head, and Carcass) (data taken from panel b). The red line is the median number. The asterisks indicate a Mann–Whitney P value < 0.001. These data are the sum of three independent biological replicates. The number of mosquitoes assayed is shown below each column

Once eL3 have developed, their intensity and prevalence are constant

To determine the optimal day to perform the emergence assay, we wanted to identify a time point at which eL3 recovery was maximized but mosquito mortality was still minimal. To do this, we infected populations ranging from 432 to 565 individuals, and then removed groups of approximately 50 mosquitoes on consecutive days for an emergence assay. Data from four independent experiments were pooled since it was not possible to obtain all time points from a single infection. We assessed the variation in eL3 number over the 10-day period from 12 to 21 dpi. The main emergence phase started at 13 dpi, as we observed only a single eL3 in 48 mosquitoes at 12 dpi. Once L3 begin to emerge from mosquitoes, both the number that emerge per mosquito as well as the prevalence of mosquitoes with at least one emerging L3 are relatively constant from 13 to 21 dpi (Fig. 4). These data suggest that larvae develop synchronously and that once they reach the L3 stage, their numbers remain relatively stable over time. Beyond 13 dpi, mosquito mortality continues and eL3 prevalence or intensity is not increased, Therefore, to maintain population sizes and maximize eL3 yield we typically assay mosquitoes 14–17 dpi.

Fig. 4

The number of D. immitis eL3 from Ae. aegyptiS are constant between 13 and 21 dpi. a Graph of the average prevalence in Ae. aegyptiS of D. immitis eL3 assayed 12–21 dpi. Error bars indicate the standard deviation (SD). b Dots are the number of D. immitis eL3 from individual mosquitoes assayed from 12 to 21 dpi. This experiment was performed four times. Two replicates were assayed on 12 to 18 dpi; the other two replicates were assayed on 14 to 21 dpi. Each replicate was performed with approximately 50 mosquitoes. The replicates on 12 dpi were performed with fewer mosquitoes since our preliminary data suggested that emergence was negligible on this day

Increasing the number of Dirofilaria immitis microfilariae ingested does not increase eL3 prevalence

To optimize the number of eL3 recovered from the mosquito, we next determined if increasing the number of microfilariae in the blood meal improved the recovery of eL3. For these experiments we used the standard concentration of 4000 mf/ml and included three additional concentrations of 8000, 16,000 and 32,000 mf/ml. We found that increased concentrations of microfilaria in the membrane feeder had a consequent impact on the number present in the mosquito midgut immediately after blood-feeding, with no significant difference between Ae. aegyptiS and Ae. aegyptiR (Fig. 5a). At each successive concentration, microfilariae present in the blood meal increased approximately twofold. We monitored mosquito survival for 17 days, at which time an emergence assay was performed. We chose day 17 to allow more time to monitor mosquito survival. The prevalence of eL3 in Ae. aegyptiS was not significantly different, regardless of the concentration of microfilariae fed (Fig. 5b). On a population level, the number of eL3 produced per mosquito was not increased by feeding concentrations of microfilariae greater than 4000 mf/ml (Fig. 5c). Increasing the concentration of D. immitis microfilaria used to infect Ae. aegyptiS increased mosquito mortality in a dose-dependent manner (Fig. 5d). Each increase in microfilaria concentration significantly increased mortality from the previous one, including the lowest concentration, which elevated mortality compared to those fed on uninfected blood. A similar dose–response was observed in the refractory strain; however, only the uninfected blood to 4000 mf/ml and 16,000 to 32,000 mf/ml comparisons were significantly different (Fig. 5e). When we compared the survival of Ae. aegyptiS and Ae. aegyptiR at the different concentrations of microfilariae, there was no difference in survival at the lowest concentration (Additional file 5: Figure S3). There was a modest difference at 8000 mf/ml, with Ae. aegyptiS showing greater mortality, and this difference further increased at the two highest concentrations.

Fig. 5

Increasing the dose of microfilariae does not increase numbers of eL3 but increases mosquito mortality. a Dots indicate the number of D. immitis microfilariae present in midguts of Ae. aegyptiS (blue) and Ae. aegyptiR (red) immediately following blood-feeding on the indicated doses of microfilariae. Data in each column are normally distributed, and black lines and numbers indicate the mean. No significant differences were found when Ae. aegyptiS and Ae. aegyptiR were compared at the different doses using an unpaired t-test. Data are from two independent biological replicates. b Graph of the average prevalence of D. immitis eL3 in mosquitoes feeding on blood with increasing concentrations of microfilariae, assayed 17 dpi. Error bars indicate the SD. There was no significant difference comparing the columns using analysis of variance. c Dots are the number of D. immitis eL3 from individual mosquitoes assayed 17 dpi. No significant differences were found when we compared all groups to each other or compared 4000 mf/mL to the other groups using a Kruskal–Wallis test with Dunn’s correction for multiple comparisons. Data for panels b and c are pooled from four separate biological replicates. d, e Kaplan–Meier survival plot for Ae. aegyptiS (d) or Ae. aegyptiR (e) fed with uninfected blood (BF) or blood containing different concentrations of microfilariae (4000, 8000, 16,000, 32,000 mf/ml). Pairs of adjacent treatment groups were analyzed by Kaplan–Meier, and relationships with significant differences are indicated with asterisks in Additional file 5: Figure S3 and in Additional file 6: Table S1

Stored blood containing microfilariae retains its ability to infect mosquitoes and produce eL3

All D. immitis experiments described above used freshly isolated microfilaremic blood. However, there are times when it is not possible to use this material immediately, such as when blood is shipped from another location. We wanted to compare the number of eL3 produced when mosquitoes were fed infected blood stored at 4 °C for 1 or 2 days. For these experiments, we fed mosquitoes with freshly isolated infected blood and on the next 2 consecutive days fed new cohorts with the same sample that had been stored at 4 °C. We performed an emergence assay at day 17 of each infection. There was no significant difference in the prevalence of eL3 between mosquitoes fed fresh microfilaremic blood and ones fed on an aliquot of the same blood sample stored for 1 day at 4 °C (Fig. 6a). However, there were significant decreases in eL3 prevalence in mosquitoes fed on microfilaremic blood stored for 2 days at 4° C compared to mosquitoes fed on blood stored at 4° C for 1 day and to mosquitoes fed on fresh blood. Similar trends were observed in infection intensity (Fig. 6b). Our data show that although microfilaremic blood stored at 4 °C for 2 days can still infect mosquitoes, there is a trend towards lower numbers of eL3 following blood storage, suggesting that refrigerated samples should be used as soon as possible for maximum infection potency.

Fig. 6

Infected blood stored at 4 °C produces eL3. Infected blood was used fresh (0) or after storage for 1 or 2 days (1, 2) at 4 °C. a Graph of the average prevalence of D. immitis eL3 at 17 dpi in Ae. aegyptiS. The error bar indicates the SD. The number of mosquitoes (n) analyzed is indicated for each sample. Asterisks indicate a significant difference at P < 0.05 using Fisher’s exact test. b Blue dots are the number of D. immitis eL3 emerging from individual mosquitoes assayed at 17 dpi. Asterisks indicate significant differences in intensity using Kruskal–Wallis test with Dunn’s correction for multiple comparisons (*P < 0.05; **P < 0.01). Data are pooled from two independent experiments

Emergence assay works in a natural vector of Dirofilaria immitis

Since Ae. aegypti is not considered to be an important natural vector of D. immitis, we wanted to determine whether eL3 could be obtained from a mosquito species associated with D. immitis transmission. For these experiments we used a strain of Ae. albopictus isolated from Keyport, NJ, USA (Ae. albopictusNJ). We found that eL3 were present at 17 dpi, but their prevalence and number were lower than those present in Ae. aegyptiS (Fig. 7a, b) when the mosquitoes were reared and housed in our standard insectary conditions (27 °C with 80% relative humidity [RH] and a 12:12-h photoperiod). When we tested Ae. albopictusNJ reared and infected under its ideal temperature and humidity conditions (24 °C, 70% RH, and a 16:8-h [light/dark] photoperiod), the prevalence and number of eL3 were increased, although they were still lower than was typical for Ae. aegyptiS (Fig. 7c, d), likely because the strain of Ae. albopictusNJ used did not feed to repletion from an artificial membrane feeder under any conditions that we tested. Even though we were not able to make quantitative comparisons to Ae. aegyptiS, our data show that the emergence assay works with different mosquito species.

Fig. 7

Aedes albopictus supports eL3 development. a, c Graphs of the average prevalence of D. immitis eL3 emerging at 17 dpi in Ae. aegyptiS (blue bar, Ae. aegS) or Ae. albopictusNJ (purple bar, Ae. alboNJ) reared and maintained under standard insectary conditions (a) or in Ae. albopictusNJ (purple bar, Ae. alboNJ) reared and maintained at 24 °C, 70% relative humidity and 16:8-h (light/dark) photoperiod (c). Error bars indicate the SD. The number of mosquitoes (n) analyzed is indicated for each sample. b, d Blue and purple dots are the number of D. immitis eL3 emerging at 17 dpi from individual Ae. aegyptiS (Ae. aegS) or Ae. albopictusNJ (Ae. alboNJ) mosquitoes, respectively, reared and maintained under standard insectary conditions (b) or at 24 °C, 70% relative humidity and 16:8-h (light/dark) photoperiod (d)

Individual mosquito emergence assay for transmission stage Brugia malayi

To determine whether the emergence assay will be informative for enumerating eL3 for other filarial nematodes, we infected mosquitoes with B. malayi. These parasites have a shorter developmental period in the mosquito [24], so we performed our emergence assay at 12–14 dpi in both Ae. aegyptiS and Ae. aegyptiR mosquitoes. Despite taking up a similar number of microfilariae in the blood meal (Fig. 8a), no eL3 were produced by Ae. aegyptiR, showing that this strain is refractory to both B. malayi and D. immitis (Fig. 8b). In contrast, a significant proportion of Ae. aegyptiS mosquitoes developed eL3, showing that this strain is susceptible to both B. malayi and D. immitis (Fig. 8b). There was no significant difference in either the prevalence of mosquitoes producing eL3 or in the number of eL3 produced per mosquito between the days we assayed (Fig. 8b-c). These data indicate that despite their different life-cycle in the mosquito, eL3 of human filariae can be measured using our emergence assay.

Fig. 8

Emergence assay can be used to quantify B. malayi eL3. a Dots indicate the number of Brugia malayi microfilariae present in midguts of Ae. aegyptiS (blue) and Ae. aegyptiR (red) immediately following blood-feeding. Data in each column are not normally distributed; the black line is the median. The number of mosquitoes (n) analyzed is indicated for each sample. No significant difference was found using a Mann–Whitney test (P = 0.09). b Graph of the average prevalence of B. malayi eL3 assayed 12–14 dpi in Ae. aegyptiS (blue bars) and at 12 and 14 dpi in Ae. aegyptiR (red bars). Error bars indicate the SD. The number of mosquitoes (n) analyzed is indicated for each sample. No emerging parasites were observed for Ae. aegyptiR. There were no significant differences between the days assayed for Ae. aegyptiS, and all Ae. aegyptiS days assayed were significantly different from both Ae. aegyptiR on the two days assayed using an analysis of variance with Tukey’s multiple comparisons test, as indicated by asterisks (P < 0.001). c Blue dots are the number of B. malayi eL3 from individual mosquitoes assayed 12–14 dpi. No significant differences were found when all groups were compared to each other or when day 12 post infection was compared to the other groups using a Kruskal–Wallis test with Dunn’s correction for multiple comparisons. Data were pooled from three independent experiments


The development of an assay for eL3 may be valuable for studying mosquito–filaria interactions, thereby providing a clearer indication of vector competence and vector transmission intensity. As our data and a previously reported observation [5] indicate, only a portion of L3 residing in the mosquito emerge when stimulated either by warming the mosquito or by direct contact with a mammalian host, even if already residing in the head. Our method provides a more accurate indication of a particular vector species’ potential for pathogen transmission. For example, our results show that not all strains of Ae. aegypti or Ae. albopictus support eL3 development, even though microfilariae invade the Malpighian tubules. In other studies, we used this assay to show that activation of the Toll immune signaling pathway restricts development of D. immitis and B. malayi eL3 [19, 25]. In addition, this assay could also permit assessment of manipulations of the mosquito host or larvae that result in an inability of L3 to emerge in response to thermal stimuli or due to motor defects that could be missed by current methods. Finally, the results of our assays suggest that quantitating all L3 by dissection will likely result in overestimating the number of larvae that are capable of emerging from the mosquito. This is particularly true in the case where the number of L3 is derived by mosquito homogenization, as L3 from the body cavity and those present in the Malpighian tubules are likely to be included in this method.

Overall, we found that 32% of the D. immitis-infected and approximately 50% of B. malayi-infected mosquitoes develop at least one eL3, which is similar to previous observations measuring emergence of L3 [26,27,28]. Since mosquitoes typically blood-feed more than once, it is interesting to speculate that the L3 that do not emerge may enter the proboscis and emerge in a subsequent blood meal, thereby increasing the chance of transmission. On the other hand, it is also possible that the eL3 we observe are the only ones competent to emerge and infect another host. In this case, the failure of the remaining L3 to emerge could be due to competition for limited resources in the vector or a parasite strategy to control the density of L3 to limit damage to the vector.

Results of our experiments to optimize recovery of eL3 by increasing the dose of D. immitis microfilariae given to mosquitoes reveal that microfilarial uptake and eL3 emergence are uncoupled, as we did not observe significant increases in the prevalence of mosquitoes with eL3 or the number of eL3 per mosquito at the doses tested. While it is likely that microfilarial uptake and eL3 emergence are coupled at lower concentrations of microfilariae, we did not test this since our main goal was to establish conditions where eL3 recovery is maximized to support future study of transmission-blocking strategies. Varying the timing of the assay revealed that at 13 dpi there is no significant difference in the prevalence or number of eL3. Taken together, our data suggest that the Malpighian tubules have a limited capacity to support D. immitis development and that no additional eL3 are produced once the limit is reached. However, we observed a range of developmental phenotypes in the Malpighian tubules of mosquitoes 14 days after D. immitis infection, raising the possibility that larval damage to the tubules prevents further development, as all larvae are viable at this time point, even those displaying delayed development phenotypes. While a substantial number of midgut epithelial cells are invaded during infection by ookinetes of Plasmodium, the causative agent of malaria, damaged cells are eliminated and replaced through tissue regeneration [29, 30]. As larval development is blocked and mosquito fitness is negatively impacted over time, this process suggests that damaged cells of the Malpighian tubules persist and are not replaced. In addition, the continuing metabolism of the increased number of larvae or an accumulation of larval waste products may also contribute to the increased mosquito mortality we observed in Ae. aegyptiS at later timepoints.

By quantifying microfilarial uptake in individual mosquitoes and comparing it to all parasites that emerge from either the whole mosquito, the head or the carcass or to those present in the Malpighian tubules at 14 dpi, we found that approximately 60% of the ingested microfilariae are accounted for at 14 dpi. Although we are accounting for a majority of the parasites ingested by the mosquitoes, it is nevertheless interesting to speculate about the fate of those that are not assayed. Some L3 remain in the proboscis of dissected heads, even after the primary emergence assay and the subsequent emergence assay after dissection. However, we did not systematically attempt to quantify these, and it remains possible that L3 may also be retained in the dissected carcasses. In addition, because some microfilariae may be damaged by the mosquito immune system or fail to follow sensory cues, they may fail to invade the Malpighian tubules and may be voided into the hindgut and then the feces [4, 31, 32]. Likewise, the activity of microfilariae and larvae in the Malpighian tubule cells may damage these cells, sometimes to the point where microfilariae are released into the tubule lumen, where they also could be eliminated as waste. Alternatively, if the basal side of the Malpighian tubule cell is compromised, parasites could be released into hemolymph within the mosquito body cavity, where they could be eliminated or sequestered. As the possibilities outlined above are not mutually exclusive, we believe they could collectively account for the differential between microfilarial uptake and total parasites ultimately detected. Interestingly, it was recently shown using field populations of Ae. albopictus, a natural vector of D. immitis, that in areas of greater infection prevalence, larval damage to the mosquito is better tolerated, benefitting both the vector and the parasite [33].

We used our emergence assay to analyze the effects of storing microfilaremic blood at 4 °C and showed that it is possible to produce eL3 after a storage time of at least 2 days, but likely even longer. However, while delays in initiating mosquito infection do not preclude experimentation, the strongest prevalence and intensity of eL3 production was observed in mosquitoes infected through the ingestion of fresh microfilaremic blood. Given the loss of eL3 production with blood storage time, it is not recommended to make comparisons within an experiment using a blood sample stored for different lengths of time. However, internal comparisons are reasonable, as is the goal of using the stored blood to produce eL3.

Because L3 obtained in our assay have responded to physiological conditions, L3 produced via an emergence assay may provide a more easily accessible source of infective larvae than L3 obtained from gently crushed and sieved mosquitoes [34]. While we developed this emergence assay for use on single mosquitoes, it is also suitable for use on populations en masse, and eL3 obtained this way are known to be infective [17]. As such, eL3 may be quite valuable for future identification and testing of novel heartworm preventatives, which requires infectious D. immitis L3, as well as for studies of the host immune response to infection, which often require infectious L3. Similarly, in vitro L3 to L4 molting assays, such as the newly developed genetic transformation protocol for B. malayi [35], may benefit from L3 produced using our method. Finally, given the widespread nature of vector-borne filarial diseases and their potential to spread due to changing environmental conditions, new methods like this could help assess transmission potential in the field and to develop methods in the laboratory to block transmission. This easy, efficient and cost-effective method has the potential to be a valuable tool for the quantitative analysis of mosquito transmission of filariae, especially to researchers in countries most affected by these parasites where resources are often constrained.


We have established a novel assay to determine the number of infectious L3 filarial larvae capable of emerging from individual mosquitoes, which we refer to as eL3. We have shown this assay works with both different mosquito and filarial nematode species. As such, our method is likely to be suitable for assessment eL3 of other mosquito transmitted filariae, such as Dirofilaria repens, a canine and human skin-dwelling relative of D. immitis, and Wuchereria bancrofti, which is responsible for approximately 90% of human lymphatic filariasis and can be transmitted by several genera of mosquitoes (Culex, Aedes and Anopheles). It remains to be determined if our assay will work for filariae transmitted by other arthropod vectors, such as biting flies, mites, fleas and ticks. In summary, the method we describe here will greatly facilitate current efforts to block transmission of arthropod transmitted filariae by enabling quantitative analysis in the vector as well as providing a more reliable way to harvest infectious larvae to evaluate new preventatives, treatments or vaccines.

Availability of data and materials

All data generated or analyzed during this study are included in this published article and its supplementary information files.


BE, susceptible, Ae. aegypti S :

Aedes aegypti Blackeye Liverpool strain

LVP, refractory, Ae. aegypti R :

Aedes aegypti Liverpool strain




Malpighian tubules


Third-stage larvae


Emerging third-stage larvae


  1. 1.

    Taylor MJ, Hoerauf A, Bockarie M. Lymphatic filariasis and onchocerciasis. Lancet. 2010;376(9747):1175–85.

    Article  PubMed  PubMed Central  Google Scholar 

  2. 2.

    Companion Animal Parasite Council. 2012. Accessed Dec 2019.

  3. 3.

    McCall JW, Genchi C, Kramer LH, Guerrero J, Venco L. Heartworm disease in animals and humans. Adv Parasitol. 2008;66:193–285.

    Article  PubMed  Google Scholar 

  4. 4.

    Beerntsen BT, James AA, Christensen BM. Genetics of mosquito vector competence. Microbiol Mol Biol Rev. 2000;64(1):115–37.

    CAS  Article  Google Scholar 

  5. 5.

    McGreevy PB, Theis JH, Lavoipierre MM, Clark J. Studies on filariasis. III. Dirofilaria immitis: emergence of infective larvae from the mouthparts of Aedes aegypti. J Helminthol. 1974;48 4:221–8.

  6. 6.

    Bradley TJ, Nayar JK. An ultrastructural study of Dirofilaria immitis infection in the Malpighian tubules of Anopheles quadrimaculatus. J Parasitol. 1987;73(5):1035–43.

    CAS  Article  Google Scholar 

  7. 7.

    McKay T, Bianco T, Rhodes L, Barnett S. Prevalence of Dirofilaria immitis (Nematoda: Filarioidea) in mosquitoes from northeast Arkansas, the United States. J Med Entomol. 2013;50(4):871–8.

    Article  PubMed  Google Scholar 

  8. 8.

    Ledesma N, Harrington L. Mosquito vectors of dog heartworm in the United States: vector status and factors influencing transmission efficiency. Top Companion Anim Med. 2011;26(4):178–85.

    Article  PubMed  Google Scholar 

  9. 9.

    Laney SJ, Ramzy RM, Helmy HH, Farid HA, Ashour AA, Weil GJ, et al. Detection of Wuchereria bancrofti L3 larvae in mosquitoes: a reverse transcriptase PCR assay evaluating infection and infectivity. PLoS neglected tropical diseases. 2010;4(2):e602;

  10. 10.

    Blagburn BL, Arther RG, Dillon AR, Butler JM, Bowles JV, von Simson C, et al. Efficacy of four commercially available heartworm preventive products against the JYD-34 laboratory strain of Dirofilaria immitis. Parasites Vectors. 2016;9:191.

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  11. 11.

    Bowman DD, McTier TL, Adams EL, Mahabir SP, Login JA, Bidgood T, et al. Evaluation of the efficacy of ProHeart® 6 (moxidectin) against a resistant isolate of Dirofilaria immitis (JYD-34) in dogs. Parasites Vectors. 2017;10(Suppl 2):502.

  12. 12.

    Kryda K, Six RH, Walsh KF, Holzmer SJ, Chapin S, Mahabir SP, et al. Laboratory and field studies to investigate the efficacy of a novel, orally administered combination product containing moxidectin, sarolaner and pyrantel for the prevention of heartworm disease (Dirofilaria immitis) in dogs. Parasites Vectors. 2019;12(1):445;

  13. 13.

    Lok JB, Mika-Grieve M, Grieve RB. Cryopreservation of Dirofilaria immitis microfilariae and third-stage larvae. J Helminthol. 1983;57(4):319–24.

    CAS  Article  PubMed  Google Scholar 

  14. 14.

    Marcombe S, Farajollahi A, Healy SP, Clark GG, Fonseca DM. Insecticide resistance status of United States populations of Aedes albopictus and mechanisms involved. PLoS One. 2014;9 7:e101992;

  15. 15.

    Povelones M, McCrea AR. Infecting and mosquitoes with Dirofilaria immitis and Brugia malayi. 2020; doi: 10.17504/

  16. 16.

    Povelones M, McCrea AR. Dirofilaria immitis and Brugia malayi emergence assay for individual or pools of mosquitoes. 2020; doi: 10.17504/

  17. 17.

    Lok JB, Knight DH, Wang GT, Doscher ME, Nolan TJ, Hendrick MJ, et al. Activity of an injectable, sustained-release formulation of moxidectin administered prophylactically to mixed-breed dogs to prevent infection with Dirofilaria immitis. Am J Vet Res. 2001;62(11):1721–6.

    CAS  Article  Google Scholar 

  18. 18.

    Lok JB, Mika-Grieve M, Grieve RB, Chin TK. In vitro development of third- and fourth-stage larvae of Dirofilaria immitis: comparison of basal culture media, serum levels and possible serum substitutes. Acta Trop. 1984;41(2):145–54.

    CAS  PubMed  Google Scholar 

  19. 19.

    Edgerton EB, McCrea AR, Berry CT, Kwok JY, Thompson LK, Watson B, et al. Activation of mosquito immunity blocks the development of transmission-stage filarial nematodes. Proc Natl Acad Sci USA. 2020.

    Article  PubMed  Google Scholar 

  20. 20.

    Kartman L. Factors influencing infection of the mosquito with Dirofilaria immitis (Leidy, 1856). Exp Parasitol. 1953;2(1):27–78.

    Article  Google Scholar 

  21. 21.

    McGreevy PB, McClelland GA, Lavoipierre MM. Inheritance of susceptibility to Dirofilaria immitis infection in Aedes aegypti. Ann Trop Med Parasitol. 1974;68(1):97–109.

    CAS  Article  Google Scholar 

  22. 22.

    Nayar JK, Knight JW, Bradley TJ. Further characterization of refractoriness in Aedes aegypti (L.) to infection by Dirofilaria immitis (Leidy). Experimental parasitology. 1988;66(1):124–31.

  23. 23.

    Sauerman DM Jr, Nayar JK. Characterization of refractoriness in Aedes Aegypti (Diptera: Culicidae) to infection by Dirofilaria immitis. J Med Entomol. 1985;22(1):94–101.

    Article  PubMed  Google Scholar 

  24. 24.

    Erickson SM, Xi Z, Mayhew GF, Ramirez JL, Aliota MT, Christensen BM, et al. Mosquito infection responses to developing filarial worms. PLoS Negl Trop Dis. 2009;3 10:e529;

  25. 25.

    McCrea AR, Jimenez Castro PD, Kaplan RM, Povelones M. Activation of the Toll pathway in Aedes aegypti blocks the development of emerging third-stage larvae of drug-resistant Dirofilaria immitis. Vet Parasitol. 2020.

    Article  PubMed  Google Scholar 

  26. 26.

    Grieve RB, Lok JB, Glickman LT. Epidemiology of canine heartworm infection. Epidemiol Rev. 1983;5:220–46.

    CAS  Article  PubMed  Google Scholar 

  27. 27.

    Gasarasi DB. The transmission dynamics of bancroftian filariasis: the distribution of the infective larvae of Wuchereria bancrofti in Culex quinquefasciatus and Anopheles gambiae and its effect on parasite escape from the vector. Trans R Soc Trop Med Hyg. 2000;94(3):341–7.

    CAS  Article  PubMed  Google Scholar 

  28. 28.

    Paily KP, Hoti SL, Manonmani AM, Balaraman K. Longevity and migration of Wuchereria bancrofti infective larvae and their distribution pattern in relation to the resting and feeding behaviour of the vector mosquito Culex quinquefasciatus. Ann Trop Med Parasitol. 1995;89(1):39–47.

    CAS  Article  PubMed  Google Scholar 

  29. 29.

    Han YS, Barillas-Mury C. Implications of time bomb model of ookinete invasion of midgut cells. Insect Biochem Mol Biol. 2002;32(10):1311–6.

    CAS  Article  Google Scholar 

  30. 30.

    Vlachou D, Zimmermann T, Cantera R, Janse CJ, Waters AP, Kafatos FC. Real-time, in vivo analysis of malaria ookinete locomotion and mosquito midgut invasion. Cell Microbiol. 2004;6(7):671–85.

    CAS  Article  Google Scholar 

  31. 31.

    Christensen BM. Observations on the immune response of Aedes trivittatus against Dirofilaria immitis. Trans R Soc Trop Med Hyg. 1981;75(3):439–43.

    CAS  Article  Google Scholar 

  32. 32.

    Bartholomay LC. Infection barriers and responses in mosquito–filarial worm interactions. Curr Opinion Insect Sci. 2014;3:37–42.

    Article  Google Scholar 

  33. 33.

    Dharmarajan G, Walker KD, Lehmann T. Variation in tolerance to parasites affects vectorial capacity of natural Asian tiger mosquito populations. Curr Biol. 2019;29(22):3946-52.e5.

  34. 34.

    Evans CC, Moorhead AR, Storey BE, Blagburn BL, Wolstenholme AJ, Kaplan RM. Evaluation of the larval migration inhibition assay for detecting macrocyclic lactone resistance in Dirofilaria immitis. Vet Parasitol. 2017;246:76–81.

    CAS  Article  PubMed  Google Scholar 

  35. 35.

    Liu C, Mhashilkar AS, Chabanon J, Xu S, Lustigman S, Adams JH, et al. Development of a toolkit for piggyBac-mediated integrative transfection of the human filarial parasite Brugia malayi. PLoS Negl Trop Dis. 2018;12(5):e0006509.

  36. 36.

    Bancroft TL. Report LXXXV: Some further observations on the life-history of Filaria Immitis Leidy. Br Med J. 1904;1(2258):822–3.

    CAS  Article  Google Scholar 

Download references


We thank Leslie King who helped with the critical reading of the manuscript and the Filariasis Research Reagent Resource center for providing Brugia malayi and the Aedes aegypti Black Eye Liverpool strain.


This work was supported by a University Research Foundation grant (URF-2017), intramural funds, and NIH grant AI139060 to MP. JBL was supported by NIH grants AI050668 and AI44572.

Author information




MP was responsible for the study conception. ARM, EBE, GTO, FMO and MP were responsible for acquisition of data. ARM, EBE, GTO, FMO, TJN, JBL and MP were responsible for the analysis and interpretation of data. MP and ARM were responsible for drafting and critical revision of the manuscript. EBE, GTO, FMO, TJN and JBL were responsible for critical revision of the manuscript. All authors read and approved the final manuscript.

Corresponding author

Correspondence to Michael Povelones.

Ethics declarations

Ethics approval and consent to participate

Blood containing D. immitis microfilariae was obtained from an experimentally infected dog according to Institutional Animal Care and Use Committee approved protocols and in accordance with the guidelines of the Institutional Animal Care and Use Committee of the University of Pennsylvania (IACUC, protocol 805059).

Consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interests.

Additional information

Publisher's Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Additional file 1: Movie 1.

Third-stage larvae visible moving in the proboscis of Ae. aegyptiS 14 days after infection with D. immitis.

Additional file 2: Figure S1.

Mosquito dissection for analysis after emergence assay. After the emergence assay from the whole body (a), the head (b) and carcass (c) were placed individually into separate wells. The number of L3 larvae emerging from the dissected head and carcass were assayed after incubation at 37 °C. The Malpighian tubules were removed from the carcass prior to placing it in the well. Mosquito after removing head with fine forceps (d) and carcass after the Malpighian tubules (arrow) are dissected out (e). The scale bars in a–c and d, e are 500 and 1000 µm, respectively.

Additional file 3: Movie 2.

Two eL3 in a well of a 96-well plate following an emergence assay performed on Ae. aegyptiS 14 days after infection with D. immitis. Another eL3 is visible at the top of the frame.

Additional file 4: Figure S2.

Example of D. immitis larval lengths scored in Malpighian tubules. Malpighian tubules dissected following an emergence assay contain viable larvae of different lengths indicated with asterisks. Different stage larvae are typically present.

Additional file 5: Figure S3.

Ae. aegyptiS have greater mortality than Ae. aegyptiR following D. immitis infection. Pairs of adjacent treatment groups from Fig. 5d, e were analyzed by Kaplan–Meier and relationships, with significant differences indicated with asterisks here and in Additional file 6: Table S1. Aedes aegyptiS and Ae. aegyptiR are indicated in blue and red, respectively.

Additional file 6: Table S1.

Pairwise comparisons of mosquito survival following blood feeding on different doses of D. immitis microfilariae.

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit The Creative Commons Public Domain Dedication waiver ( applies to the data made available in this article, unless otherwise stated in a credit line to the data.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

McCrea, A.R., Edgerton, E.B., Oliver, G.T. et al. A novel assay to isolate and quantify third-stage Dirofilaria immitis and Brugia malayi larvae emerging from individual Aedes aegypti. Parasites Vectors 14, 30 (2021).

Download citation


  • Aedes aegypti
  • Aedes albopictus
  • Dirofilaria immitis
  • Brugia malayi
  • Mosquito
  • Filaria
  • Transmission