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Aquatain® causes anti-oviposition, egg retention and oocyte melanization and triggers female death in Aedes aegypti

Parasites & Vectors volume 15, Article number: 100 (2022) Cite this article

Abstract

Background

In arboviral disease systems where the virus can be transmitted from male to female vectors and from one generation to the next, targeting the female (especially when she is gravid) can help alter the persistence of the virus in nature and its transmission. A typical example is Aedes aegypti, which has become unmanageable due to the development of insecticide resistance. Despite evidence that monomolecular surface films prevent the selection of genetic resistance, their potential in Aedes vector control remains largely unexplored.

Methods

We examined the oviposition, egg retention, oocyte melanization, and female mortality of the Cayman Islands strain of Ae. aegypti, using choice (balanced and unbalanced) and no-choice bioassays involving Aquatain® Mosquito Formulation (AMF; Aquatain Products Pty Ltd.), a polydimethylsiloxane–based liquid used for mosquito control.

Results

When presented with similar opportunities to oviposit in two sites treated with AMF and two other sites with untreated water (control), egg deposition rates were significantly higher in the untreated water sites than in the AMF-treated sites (P < 0.05). We also observed a matching pattern of egg deposition preference in environments with more options in terms of AMF-treated sites. Females laid significantly more eggs when water was the only available medium than when all sites were treated with AMF (P < 0.05). Also, significantly more mature eggs were withheld in the AMF no-choice environment than in the no-choice test involving only water (P < 0.05). Internal oocyte melanization was not observed in females from the oviposition arenas with the lowest AMF presence (equal-choice and water-based no-choice); in contrast, this physiological response intensified as the number of AMF-treated sites increased. Female death occurred at high rates in AMF-treated environments, and this response increased with the increasing presence of such egg deposition sites.

Conclusions

This study demonstrated that AMF acted as a deterrent signal to ovipositing Ae. aegypti and as an indirect adulticide. These results suggest that AMF may be a promising control tool against the dengue vector, and this warrants further evaluation under field settings.

Graphical Abstract

Background

Despite several decades of control efforts, mosquito vectors and the diseases they transmit still represent significant threats to human health [1, 2]. Beyond disease transmission, mosquitoes represent a serious menace to human quality of life [3] and economic development [4]. This is the case for most Caribbean islands [5], as demonstrated by an unprecedented epidemic of chikungunya and Zika viruses and febrile illness due to dengue in recent years [6]. These public health threats, in particular, the link between the Zika virus and reproductive health, pregnancy and congenital disabilities [7,8,9], have stimulated interest in Aedes aegypti, the primary vector of all the above-mentioned viruses [10].

Efforts to prevent outbreaks of these diseases have mostly counted on the use of insecticides, but success has been limited due to the development of insecticide resistance [11, 12]. Apart from increased resistance to the four existing families of adulticides, namely pyrethroids, organophosphates, carbamates and organochlorines [13, 14], the control of Ae. aegypti with larvicides is hindered by a reduced susceptibility [15], international scrutiny and deregulation due to toxicity against biodiversity [16] and the existence of inconspicuous larval habitats [17, 18].

Female Ae. aegypti disperse eggs across multiple natural and artificial containers associated with human activity [19,20,21]. Despite this multitude of potential breeding sites, Ae. aegypti has been reported to successfully locate those that can guarantee the success of the offspring and to ignore others that are unsuitable for larval development completion [22,23,24]. This ability to identify high-quality oviposition sites and select those that provide increased larval performance is mediated by many parameters, but most studies have focused on the role of olfactory cues [25] and habitat physics [20]. However, while some studies have specifically analyzed components of the site's physical structure that affect egg deposition choice [26], there has been little research on the physical features of water bodies, which are known to present several visual signals [20], such as texture and reflectance from the water surface; these cues have been reported to influence the oviposition of container-breeding mosquitoes, including Ae. aegypti [27,28,29,30].

Surface tension is a property of water that plays an integral part in the development and survival of aquatic insects, including mosquitoes [31, 32]. Surface tension can be generated when a water surface is covered with an oil film [33, 34]; in this situation, the oil film elicits an elastic behavior in the water, causing it to acquire as small a surface area as possible [35]. This reduction in surface tension produces a film at the air–water interface [20]. Adult Aedes aegypti prefer a high level of surface tension and are incapable of resting on a water surface with a reduced tension [36]; specifically, it exhibits high mortality responses by drowning when exposed to water with reduced surface tension [36].

In addressing dengue vector control, the World Health Organization [37] and many other scientists studying mosquitoes [23, 38] have called for oviposition to be taken into account, not only because of transovarial transmission of viruses [39] but also because preventing oviposition can disrupt the life-cycle of the mosquito and thereby reduce population growth [23]. Due to these potentially positive control outcomes, some studies have addressed the use of oil to prevent mosquito oviposition, but most of these investigations have used either essential oils [40,41,42], lecithin monolayers [43,44,45] or Agnique MMF, a monomolecular surface film formulation (Cognis Corp., Cincinnati, OH, USA) [46], all of which are known to be easily broken down by wind and rainfall [47, 48]. In a recent study [49] that has tested an oil film with high resilience to being broken down by wind and rain, namely Aquatain® Mosquito Formulation (AMR; Aquatain Products Pty Ltd, Dandenong South, VIC, Australia [50]), the authors did not specifically address oviposition and Ae. aegypti. In the present study, we assessed the oviposition, egg retention, oocyte melanization, and female mortality of Ae. aegypti in response to the presence of different levels of AMF in potential breeding sites.

Methods

Colony maintenance

The Ae. aegypti mosquitoes used in this study were from a colony maintained at the insectarium of the Mosquito Research and Control Unit (MRCU; George Town, Cayman Islands) and maintained at 26.5 ± 1 °C, 65 ± 4% relative humidity, and a photoperiod of 13:10 h (light:dark) with 1 h of dusk. The colony originated from larvae collected from different containers in George Town in November 2020. The larvae were standardly reared in plastic trays with 800 ml tap water containing 100– 150 larvae. Larval food (ground Tetramin; Tetra, Melle Germany) was supplied once daily, and the rearing medium was replaced with fresh water prior to each third feeding [24]. Pupae were placed in polystyrene cups (50-ml capacity) and transferred to BugDorm cages (30 × 30 × 30 cm; MegaView Science Co., Ltd., Taichung, ROC [Taiwan]). Emerging adults had continuous access to 10% sucrose solution. Females were artificially offered blood meals once every 2 weeks. Three days after blood-feeding, eggs were collected, air-dried under insectary conditions and stored for colony maintenance or experiments.

Experimental specimens

To obtain gravid females, egg samples from the colony stock were submerged in tap water, and four larval population replicates, each with 200 newly hatched larvae, were reared as outlined in section Colony maintenance. The gravid females were fed every 2 days with Tetramin, and the rearing water of each colony was replaced with fresh water before pupation started. Pupae were held in plastic cups and transferred into cages where a 10% sugar solution was available. Three- to four-day-old females were offered blood meals for 10 min. Fully engorged females with digested blood meals for 3 days were considered to be gravid and used as experimental material.

Chemical and test concentration

The AMF used in this study contains 78% active ingredient polydimethylsiloxane (also called silicone) and was applied at 1 ml/m2, which is the application rate recommended by the manufacturer [50]. The test oviposition medium was generated with reference to the approved application rate and taking into account the dimensions of the experimental containers used in this study. Each container used as an oviposition site (depth: 7.3 cm, diameter: 3.3 cm) had a surface area of 33.16 cm2. Based on these dimensions, a volume of 3.316 µl of AMF was added to 150 ml of water, and the resulting solution was used as an oviposition medium. The control water medium had a final volume of 150 ml + 3.316 µl. For convenience, containers with the test medium or water were designated as “AQ” and “W,” respectively.

Experimental features

All oviposition tests were performed following a published experimental design [24, 51], with slight modifications. Figure 1 shows the design of the oviposition bioassay. The egg deposition space consisted of four acrylic containers (depth: 7.3 cm, diameter: 3.3 cm), each with a layer of white paper (length: 8 cm, width: 8 cm) that covered the entire surface of the container and served as an egg deposition substrate. A container was placed at each corner of the cage; to remove/minimize any likely location bias, the position of the oviposition site (i.e. the corner at which a specific container was placed) was modified in the bioassay replicates in accordance with a previously described clockwise replication blueprint [24, 51]. In this scheme, each oviposition test replicate had a designated layout regarding the four oviposition containers within the cage. All bioassay types were repeated four times, and for each replication, a batch of 12 fully blood-fed females that had digested their meals for 3 days, new egg deposition substrates and new oviposition media were used. All oviposition arenas were equipped with a sugar source supplied by a cotton wick soaked with a 10% sucrose solution. The sugar supply apparatus (cotton wick and fresh sugar solution) was replenished once during the oviposition period, which lasted 10 days. All oviposition bioassays were performed at 28 ± 2 °C and 70 ± 3% relative humidity, respectively.

Fig. 1
figure 1

Oviposition bioassay design. The containers were placed on the dish, which was positioned at the bottom center of the cage. Containers were placed such that each container was at an identical distance from the adjacent container. A bioassay replicate coincided with one arrangement of the four containers

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Bioassays

To ascertain whether or not the presence of AMF influences the oviposition responses of Ae. aegypti, we ran four consecutive bioassays (Fig. 1 [51]. In the first test, 12 gravid females were placed in a BugDorm cage (30 × 30 × 30 cm) containing an oviposition arena with four W containers (W1, W2, W3, and W4) and a sugar supply source. A second bioassay was performed, as illustrated in Fig. 1, but the 12 females were given options to lay eggs in four AQ containers (AQ1, AQ2, AQ3, and AQ4). In the third test, 12 females were given equal chances to lay eggs in two AMF-treated containers (AQ1 and AQ2) and two others with water (W1 and W2). In the fourth bioassay, 12 females were presented with more options to oviposit in AMF-treated containers (AQ1, AQ2, and AQ4) than in water (W1). Each of the tests was replicated four times, and in all bioassays, females were allowed to oviposit for 10 days.

Data collection and statistical analyses

At the end of the oviposition period, dead females were counted in each cage replicate of each bioassay type and immediately frozen alongside survivors. Egg depositions were checked in all bioassays following the procedures of Dieng et al. [51], using a stereomicroscope (Motic SMZ-171-TLED; Motic Instruments Inc.; Schertz, TX, USA). The total number of eggs laid in each container replicate was quantified by counting the eggs present on the surface of the water media, paper substrates and lower surfaces of the bottom of the containers. The resulting numbers were used to determine the percentages of eggs laid in a given oviposition container replicate using the following formula: (total number of eggs deposited in a given media divided by the total number of eggs deposited in all media of a given bioassay replicate) × 100. The mean values of numbers of eggs deposited in a given bioassay replicate were determined by summing up all numbers of eggs in a given bioassay divided by the total number of experimental females. Percentages and mean values were utilized to score oviposition responses. Non-dried females were dissected, and the two ovaries were examined for egg presence under the stereomicroscope. The number of eggs withheld was counted for each dissected female, and the number of eggs produced by a female was defined as the sum of eggs laid and retained, in accordance with Farjana and Tuno [52]. Following Dieng et al. [51], we calculated the egg retention rate for each dissected female as: (total number of eggs withheld divided by the total of eggs produced) × 100. The percentage of eggs retained by a given female was defined as: (total number of eggs retained divided by the total number of eggs produced) × 100. At each dissection, the numbers of eggs with different coloration (white/light gray; dark-gray with black spots; and black) were recorded. We considered eggs with white/light-gray, dark-grey and black coloration eggs to be non-melanized, melanizing and melanized, respectively. The number of eggs in each state was used to determine the percentages of non-melanized, melanizing and melanized eggs. The differences in oviposition, egg retention and eggshell melanization responses were analyzed by nonparametric test (Kruskal–Wallis). The Dwass-Steel-Chritchlow-Fligner test was used to assess the significance of the differences between mean values for oviposition, egg retention and eggshell melanization. Female mortality data were checked for normality using the Shapiro–Wilk test. Mortality responses were examined by analysis of variance (ANOVA) from Systat version 13 [53], and mean mortality values were separated by the Tukey–Kramer honestly significant difference (HSD) test. In all analyses, P < 0.05 indicated statistical significance.

Results

Oviposition responses to AMF-treated water at various competition levels with water

When water was the only medium available to the female mosquitoes, eggs were found in each of the four containers. Of the 2084 eggs laid, 30.13% (628/2084), 20.49% (427/2084), 22.69% (473/2084) and 26.68% (556/2084) were deposited in W1, W2, W3 and W4, correspondingly. The mean (± standard error [SE]) number of eggs deposited was 130.25 ± 21.31 per container (W1: 157.00 ± 37.68, range: 72–230; W2: 106.75 ± 45.87, range: 24–238; W3: 118.25 ± 43.59, range: 54–247; W4: 139.00 ± 56.25, range: 40–286). Egg deposition did not differ between these containers (Kruskal–Wallis test statistic: 0.746, df = 3, P = 0.862) (Fig. 2a). When given equal chances to oviposit in two containers holding water supplemented with AMF and two others with water, Ae. aegypti females laid eggs in all containers, but oviposition responses varied significantly with container medium. Of the 1185 eggs oviposited by the 12 females, 95.44% (1131/1185) were deposited in containers with water, and 4.56% (54/1185) deposited in containers with AMF-treated water. The mean egg deposition was significantly higher in containers with water (141.37 ± 10.84 eggs, range: 93–184; W1: 152.25 ± 15.19; W2: 130.50 ± 15.47) than in containers supplemented with AMF (6.75 ± 4.97 eggs, range 0–41; AQ1: 2.50 ± 0.95, range: 0–4; AQ2: 12.00 ± 9.80, range: 0–41) (Kruskal–Wallis test statistic: 11.463, df = 1, P = 0.001) (Fig. 2b). When there were more choices to lay eggs in containers with water treated with AMF, the 48 females laid 783 eggs in total, including 643 in the container with water and 140 in the three cups containing AMF, corresponding to 82.12% and 17.88% of the total eggs laid, respectively. Egg deposition was significantly lower in the presence of the oil (11.66 ± 5.13 eggs, range: 0–63; AQ1: 9.25 ± 4.38; AQ2: 6.25 ± 4.62; AQ3: 19.50 ± 14.72) than when water was the only oviposition medium (160.75 ± 50.77 eggs, range: 78–287) (Kruskal–Wallis test statistic: 8.533, df = 1, P = 0.003) (Fig. 2c). When AMF-treated containers were the only oviposition sites, Ae. aegypti deposited eggs in all four containers. A total of 540 eggs were deposited by the 48 females, of which 44.07% (238/540), 22.6% (122/540), 14.44% (78/540) and 18.88% (102/540) were oviposited in containers AQ1, AQ2, AQ3, and AQ4, respectively. Egg depositions ranged from 0 to 112 and averaged 33.75 ± 8.39 eggs per container (AQ1: 59.50 ± 25.97; AQ2: 30.50 ± 8.13; AQ3: 19.50 ± 15.65; AQ4: 25.50 ± 10.44). There were no appreciable discrepancies in oviposition response between the four containers (Kruskal–Wallis test statistic: 2.976, df = 3, P = 0.375) (Fig. 2d).

Fig. 2
figure 2

Responses of gravid Aedes aegypti females when given a choice to oviposit in four cups: a water-based no-choice, b equal choice, c more oviposition opportunities in containers with AMF-treated water, d AMF-based no-choice. Abbreviations: AMF, Aquatain® Mosquito Formulation; AQ, containers with the test medium (AMF); W, containers with water only

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Comparative oviposition responses relative to option availability and egg retention

In the water-based no-choice test, the 48 female mosquitoes (12 females per cage replicate) produced a total of 2734 eggs; the mean number of eggs laid individually was 43.43 (2084/48). The mean number of eggs laid individually was 24.68 (1185/48), 16.31 (783/48) and 11.25 (540/48) for Ae. aegypti females provided with (i) matching oviposition options and (ii) more oviposition opportunities in containers supplemented with AMF, and (iii) in the AMF-based no-choice setting, respectively. Total egg deposition when water was the only oviposition medium was 1.75-, 2.66- and 3.86-fold higher than that when half, three-fourths (3 of 4) and all (4 of 4) oviposition sites were treated with AMF, respectively (Table 1). Eggs were retained in all experimental oviposition designs (Table 2), but egg retention responses varied significantly with oviposition arena layout (Kruskal–Wallis test statistic: 23.416, df = 3, P < 0.0001). In the no-choice test involving only water, a total of 649 eggs were recovered from the ovaries of the 48 female mosquitoes at 10 days after uptake of the blood meal, indicating that these females retained 23.73% (649/2734) of their total egg production. In the equal-choice test, a total of 462 eggs were collected following dissection of the 28 surviving females at 1 week after blood digestion. When more containers were treated with the oil, a total of 1669 eggs were retained by the 41 surviving females; with 986 eggs for 38 females when containers with the oil were the only egg deposition sites. The mean number of eggs retained per female in the water-based no-choice trial (13.52 ± 3.49 eggs; range: 0–76 eggs) was appreciably lower than that in the equal-choice experiment (17.11 ± 3.99 eggs; range: 0–63 eggs) (Dwass-Steel-Chritchlow-Fligner test for pairwise comparisons [DSCF]: − 12.450, P < 0.0001), which, in turn, was substantially lower than that obtained when there were more containers treated with the oil (40.70 ± 4.88 eggs; range: 0–107 eggs; DSCF: 13.184, P < 0.0001). Individual females also retained arithmetically fewer eggs in the water-based no-choice trial than in the AMF-based no-choice trial (25.94 ± 3.98 eggs, range: 0–71 eggs), which in turn recorded significantly more eggs retained per female than in the equal-choice trial (DSCF: 9.195, P < 0.0001).

Table 1 Comparative oviposition responses of Aedes aegypti females to Aquatain® Mosquito Formulation-treated water at different levels of competition with water
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Table 2 Egg retention responses of Ae. aegypti females to Aquatain® Mosquito Formulation-treated water at different levels of competition with water
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Oocyte melanization patterns in responses to AMF exposure

Figure 3 shows the egg melanization responses and variations in melanization patterns after a 10-day oviposition period. When water was the only medium present in the oviposition arena and when there was an equal chance for oviposition in two containers with water and two others with AMF-treated water, none of the females subsequently dissected had melanized eggs. Of the 1669 eggs retained by the 41 females provided with additional oviposition opportunities in AMF-treated containers, 76.45% (1276/1669) and 15.27% (255/1669) were partially and fully melanized, respectively. When containers treated with AMF were the only oviposition sites available, 85.13% (824/968) and 14.87% (162/968) of retained eggs were moderately and fully melanized, respectively. The mean number of partially melanized eggs in the no-choice test involving AMF (21.68 ± 3.63 eggs) was lower than that when egg deposition options were biased towards containers supplemented with AMF (31.12 ± 4.86 eggs), but there was no significant discrepancy between the two mean values (DSCF: − 3.321, P = 0.087). Female mosquitoes tended to have less fully melanized eggs when all sites were treated with the oil (4.26 ± 1.44 eggs) than their counterparts maintained in the arena with the sole egg-laying option in water (6.22 ± 1.40 eggs), but the difference was not significant (DSCF: − 3.293, P = 0.092).

Fig. 3
figure 3

Melanization response patterns of the oocytes of gravid Ae. aegypti females after a 10-day exposure to AMF-treated water at various competition levels with water. a Non-melanized, b partially melanized, c fully melanized

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Mortality responses of Ae. aegypti females during oviposition in the presence of AMF

Significant differences were observed in the survival of Ae. aegypti females between the different oviposition opportunities (ANOVA: F = 12.690, df = 2, P < 0.0001; Tukey–Kramer HSD test). When containers with water were the only egg deposition sites available, the mean female mortality was 4.16 ± 4.16% and oscillated between 0 and 16.66%. Arithmetically, this latter mean was far lower than that recorded when females were given equal choices to oviposit in containers with AMF-treated water and two others with water (16.66 ± 4.16%); however, the difference was not statistically significant (Tukey–Kramer HSD test: P > 0.05). The mean mortality rate of females in the “more AMF options” experiment (42.83 ± 7.21%, range: 25–58.33%) was significantly greater than that of females in the “equal-choice experiment (Tukey–Kramer HSD test: P < 0.05) which, in turn, was numerically lower than that of females in the AMF-based no-choice test. There was no significant difference in female death when there were more options in containers holding AMF-treated water and when only containers with AMF-treated water were present (Tukey–Kramer HSD test, P > 0.05) (Fig. 4).

Fig. 4
figure 4

Mortality responses of gravid Ae. aegypti females under different oviposition conditions/arena: WBN, EQC, MAQ and AQBN. Bars with the same lowercase letter are not significantly different (P < 0.05) based on the Tukey–Kramer HSD test for means comparison. Abbreviations: AQBN, AMF-based, no-choice setting; EQC, equal-choice setting; MAQ, more AMF choices setting; WBN, water-based no-choice setting

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Discussion

The results of this study revealed significant adverse impacts of the label dose of AMF, the silicone-based monomolecular film, on Ae. aegypti. Oviposition responses were reduced with the increased presence of containers with the AMF oil. Egg retention and internal oocyte melanization rates were high in oviposition arenas dominated by the presence of containers with AMF; such effects decreased in the presence of containers with water, especially under the water-based, no-choice conditions. Death occurred at greater rates among females maintained in arenas with an increased presence of oviposition sites treated with AMF compared to arenas with an increased presence of water.

The appeal or lack of appeal (repulsiveness effect) of competitive egg deposition sites to gravid mosquito females is dictated by a diversity of factors, among which the most important is the physico-chemistry of the water medium [54] and the prospect of unfavorable conditions for larval development completion [20, 55]. Various physical elements have been shown to prevent egg deposition in mosquitoes [20, 56, 57], with water surface tension being a particularly critical factor influencing oviposition [22]. Water tension typically occurs when oil is added to water, following which the layer of water molecules and that of oil molecules achieve a balanced force between the two interfaces, causing the reduction of the surface tension at the water surface [35] and the apparition of a film [32]. Aedes aegypti has been reported to select oviposition sites that increase the possibility of larval development completion [22,23,24, 55]. In mosquitoes, the presence of an oil film on the surface of the water of potential breeding habitats has often been associated with reduced survival. For example, Mbare et al. [50], in their study of Anopheles vectors, noted a 90% larval mortality and > 80% inhibition of adult emergence at sites with an AMF film. Dawood et al. [32], working with Culex pipiens, investigated the effects of AMF on different immature stages. These authors reported significantly greater mortality rates among first-, second- and fourth-instar larvae and pupae in the treated containers than untreated ones, a result they attributed to the ability of AMF to alter the water surface tension. In a recent study, Kavran et al. [49] examined the lethality of AMF on the immature forms of two mosquito species and reported higher mortality rates among juveniles of the dengue vector, Aedes albopictus. In an earlier study, Ngrenngarmlert et al. [58] assessed the lethal potential of a silicone-based monomolecular film against Ae. aegypti and reported significant larval and pupal mortality rates. In addition to affecting the immature stages, the presence of oil can also affect the behaviors of adults [48], including ovipositing females [43]. The mechanism by which this behavioral change is effected has been well documented. According to Likura et al. [59], mosquito legs are highly hydrophobic, causing a weight-supporting force on water surfaces. For a successful egg-laying to occur, a gravid female must generate a repulsive force from the legs to be able to use the surface of the water as a foothold [58, 59] and evaluate its quality [20]. However, when silicone oil is layered over the water surface, it generates an attractive capillary force that drags the legs towards the water [58], inducing a short contact time and an escape response [59]. A shortened contact time and startle behavior will result in an incomplete exploration of the quality of the oviposition site and thus a decreased probability of egg deposition.

Two colorless oviposition media were used in the present study: AMF-treated water (150 ml of water + 3.316 µl AMF) and water (150 ml + 3.316 µl). All of the containers used in oviposition bioassays had a similar configuration, and no food was added to any container; as such, differences in oviposition responses due to a difference in study configuration is unlikely. Based on earlier reports and our methodology, the observed low oviposition responses in AMF-treated containers could be explained by an attempt of the gravid females to maximize survival of both offspring and themselves. It is possible that the ovipositing Ae. aegypti females associated the presence of AMF with poor nutritional quality and reduced chances of larval development completion. It is also likely that AMF reduced the water surface tension, which in turn prevented gravid females from either landing or staying long enough on the surfaces of the medium in the container to release their eggs.

The egg retention rates in Ae. aegypti females placed in environments dominated by the presence of containers treated with AMF were far higher than those of females kept in arenas with only water as oviposition medium. Several studies have reported egg retention in mosquitoes relative to characteristics of oviposition. Chadee et al. [60], working with  Ae. aegypti, reported increased egg retention behavior at 7 days post-blood meal when females were not provided with egg-laying substrates.

In their study of a dengue vector, Satho et al. [24] assessed changes in its oviposition responses in no-choice and choice bioassays involving different concentrations of coffee extract. These authors observed that Ae. albopictus females withheld increased numbers of mature eggs when the experimental cups containing a highly concentrated extract were the only available sites. Seenivasagan et al. [23] reported that the topical repellent diethyl phenylacetamide deterred egg depositions by Ae. aegypti females, which then retained around half of their egg production. Xue and colleagues [61] investigated oviposition behaviors in Ae. albopictus in response to DEET (diethyltoluamide) and noted that the females retained high numbers of mature eggs. Bibbs et al. [62] observed that when egg deposition sites were contaminated with a fast-acting pyrethroid insecticide (Transfluthrin), gravid females of dengue vectors withheld almost half of their eggs. Seenivasagan et al. [23] and Bibbs et al. [62] tested Ae. aegypti and reported 49% and 50% oviposition deterrence, respectively. In the present study, we looked at the effect of AMF on Ae. aegypti females and obtained egg retention rates ranging from 64.61% to 68.06%, which represent deterrence outcomes similar to those in the above-mentioned studies. Egg retention comes with many disadvantageous physiological and behavioral effects [63], including egg resorption [64], initiation of subsequent vitellogenic cycle [65], morphological changes in the follicle [66] and changes in the visual, olfactory and tactile responses of mosquitoes [67] and egg dissemination pattern [60].

Although we did not assess these effects, our study revealed some information on melanization, which is known to play various crucial roles in insects [68]. There was a clear link between oviposition medium type and eggshell melanization level. No oocyte melanization occurred when gravid females were exposed to an equal number of containers of water or AMF-treated water (i.e. equal balance between media). In contrast, eggs dissected from the ovaries of females exposed to an increased number of containers containing AMF-treated water (vs water only) showed a high prevalence of melanized eggs; while the retained eggs of mosquitoes exposed exclusively to AMF-treated water exhibited different levels of melanization (whitish/light gray [non-melanized]; dark-gray with black spots [partially melanized]; and black [fully melanized]). In dengue vectors, this biochemical process [69] generally starts after oviposition [70, 71]. Newly laid eggs that are whitish and smooth [72] undergo a melanization/sclerotization process [73] to become gradually black and hard after 2 to 4 h [72, 74, 75]. During the process, a cascade of enzymatic synthesis and activities involving the phenoloxidase [75] and DOPA decarboxylase [70, 76] lead to the production of melanin. Isoe et al. [71] recently assessed the genetic aspects of melanogenesis in Ae. aegypti and found that the eggshell organizing factor 1 (EOF1) plays an essential role in melanization. These authors suggested that partial melanization prior to oviposition is caused by the loss of EOF1 activity, which alters the chemical balance within the oocytes, which in turn activates other eggshell components to initiate the melanization process prematurely. They also noted that EOF1-deficient mosquitoes have eggs with different melanization levels, varying from non-melanized to completely melanized eggshells. In the present study, gravid Ae. aegypti females were presented with AMF-treated water as oviposition medium at different competition levels with water for the same length of time (10 days).

Although we did not investigate these phenomena, contingent on the findings of these previous studies, we presume that the synthesis and levels of phenoloxidase and decarboxylase were high in the eggs of females exposed solely to AMF-treated water and when three of the four oviposition containers contained AMF. It is plausible that the observed disparities in melanization levels between eggs in females exposed to AMF-treated water and eggs in non-exposed/less-exposed females occurred due to the high activity levels of these enzymes. This effect of AMF treatment on the activities of phenoloxidase and decarboxylase was possibly less marked in females with no (water treatment) or reduced exposure (equal-choice and three-fourths [3 of 4] of treatments) to AMF. It is also conceivable that the females exposed solely to AMF-treated water had a higher EOF1 expression level and activity. During the 10-day oviposition period, the mortality rates of gravid females were high in arenas with an increased presence of AMF-treated oviposition containers, especially the “AMF-based no-choice treatment”, compared to the “water-based no-choice treatment,” thus indicating the presence of adulticidal factors in the AMF medium. AMF is a polydimethylsiloxane (PDMS, 80%)-based liquid that is not toxic [32], as indicated by its certification for use in drinking water [77, 78]; therefore, death due to toxic chemicals is unexpected. The observed differences in female mortality responses may have been due to at least two factors. First, reducing the water surface tension in the AMF-treated containers, particularly in the AMF-based no-choice and three-fourths treatments, may have produced strong, attractive capillary forces that dragged the legs of females towards the water, consequently increasing the likelihood of sinking and death. In support of this possibility, on the surface of the water, but not on the surface of water with a silicone oil film layer, female mosquitoes can use the surface as a foothold to lay their eggs, using a maximal repulsive force from their legs [59]. Second, the untimely internal oocyte melanogenesis during egg retention may have induced the production and accumulation of toxic compounds among females with increased exposure to AMF-treated water, which in turn raised the possibility of intoxication. In favor of this contention, it has been shown that phenoloxidase activity in the insect hemolymph can produce quinonoid toxic compounds [79] and that melanin and its quinone intermediates are toxic to hosts [70].

Conclusions

We observed that treating all, three of four or half (2 of 4) of potential breeding sites of Ae. aegypti in a given environment with AMF altered the potential contribution of the site to the next generation. AMF treatment prevented females from laying sizeable numbers of eggs and caused increased egg retention and internal egg melanogenesis, all of which are conducive to the lack of reproductive success. The application of AMF in potential developmental sites also triggered the death of gravid females, thus denoting the adulticidal potential of this film. It is clear that AMF performed as an oviposition deterrent and as an indirect killer of ovipositing A. aegypti females; this latter observation would be a supplemental benefit to vector control programs. These attributes, coupled with its previously recognized direct lethality on the immature stages of dengue vectors [49, 58], advocate for the incorporation of AMF into integrated approaches for dengue vector control. As AMF is safe for humans [50, 77, 78], its use in domestic areas where Ae. aegypti thrives naturally may be widely accepted. In addition, as the mode of action of AMF is physical, its use and rotation with other larvicides can help mitigate insecticide resistance issues.

Availability of data and materials

The data supporting the results of this paper are available upon request.

References

  1. Tyagi BK. Advances in vector mosquito control technologies, with particular reference to herbal products. In: Veer V, Gopalakrishnan R, editors. Herbal insecticides, repellents and biomedicines: effectiveness and commercialization. New Delhi: Springer India; 2016. p. 1–9. https://doi.org/10.1007/978-81-322-2704-5_1.

    Chapter  Google Scholar 

  2. Rúa AV, Okech BA. The spread of mosquito-borne diseases: a major and global public health problem. In: Picimbon J-F, editor. Olfactory concepts of insect control—alternative to insecticides: volume 1. Cham: Springer International Publishing; 2019. p. 1–27. https://doi.org/10.1007/978-3-030-05060-3_1.

    Chapter  Google Scholar 

  3. Halasa YA, Shepard DS, Fonseca DM, Farajollahi A, Healy S, Gaugler R, et al. Quantifying the impact of mosquitoes on quality of life and enjoyment of yard and porch activities in New Jersey. PLoS ONE. 2014;9:e89221.

    PubMed  PubMed Central  Google Scholar 

  4. Giesen C, Roche J, Redondo-Bravo L, Ruiz-Huerta C, Gomez-Barroso D, Benito A, et al. The impact of climate change on mosquito-borne diseases in Africa. Path Glob Health. 2020;114:287–301.

    Google Scholar 

  5. Valentine MJ, Ciraola B, Jacobs GR, Arnot C, Kelly JK, Murdock CC. Effects of seasonality and land use on the diversity, relative abundance, and distribution of mosquitoes on St. Kitts, West Indies. Parasit Vectors. 2020;13:543.

    PubMed  PubMed Central  Google Scholar 

  6. Lowe R, Ryan SJ, Mahon R, Van Meerbeeck CJ, Trotman AR, Boodram LG, et al. Building resilience to mosquito-borne diseases in the Caribbean. PLoS Biol. 2020;18:e3000791.

    CAS  PubMed  PubMed Central  Google Scholar 

  7. Hennessey M, Fischer M, Staples JE. Zika virus spreads to new areas—region of the Americas, May 2015–January 2016. Morb Mortal Wkly Rep. 2016;2016:55–8.

    Google Scholar 

  8. Centers for Disease Control and Prevention (CDC). Zika virus. Atlanta: US Department of Health and Human Services, CDC; 2016. http://www.cdc.gov/zika/index.html. Accessed 20 Nov 2021.

  9. Trotman AR, Mahon R, Shumake-Guillemot J, Lowe R, Stewart-Ibarra AM. Strengthening climate services for the health sector in the Caribbean. Bulletin World Meteorology; 2018. https://public.wmo.int/en/resources/bulletin/strengthening-climate-services-health-sector-caribbean. Accessed 20 Nov 2021.

  10. Powell JR. Mosquito-borne human viral diseases: why Aedes aegypti? Am J Trop Med Hyg. 2018;98:1563–5.

    PubMed  PubMed Central  Google Scholar 

  11. Dusfour I, Vontas J, David JP, Weetman D, Fonseca DM, Corbel V, et al. Management of insecticide resistance in the major Aedes vectors of arboviruses: advances and challenges. PLoS Neglect Trop Dis. 2019;13: e0007615.

    Google Scholar 

  12. Wilke ABB, Vasquez C, Carvajal A, Ramirez M, Cardenas G, Petrie WD, et al. Effectiveness of adulticide and larvicide in controlling high densities of Aedes aegypti in urban environments. PLoS ONE. 2021;16:e0246046.

    CAS  PubMed  PubMed Central  Google Scholar 

  13. Martianasari R, Hamid PH. Larvicidal, adulticidal, and oviposition-deterrent activity of Piper betle L. essential oil to Aedes aegypti. Vet World. 2019;12:367–71.

    CAS  PubMed  PubMed Central  Google Scholar 

  14. Gan SJ, Leong YQ, Bin Barhanuddin MFH, Wong ST, Wong SF, Mak JW, et al. Dengue fever and insecticide resistance in Aedes mosquitoes in Southeast Asia: a review. Parasit Vectors. 2012;14:315.

    Google Scholar 

  15. Bisset JA, Rodríguez MM, Piedra LA, Cruz M, Gutiérrez G, Ruiz A. Reversal of resistance to the larvicide temephos in an Aedes aegypti (Diptera: Culicidae) laboratory strain from Cuba. J Med Entomol. 2020;57:801–6.

    CAS  PubMed  Google Scholar 

  16. Marcombe S, Chonephetsarath S, Thammavong P, Brey PT. Alternative insecticides for larval control of the dengue vector Aedes aegypti in Lao PDR: insecticide resistance and semi-field trial study. Parasit Vectors. 2018;11:616.

    CAS  PubMed  PubMed Central  Google Scholar 

  17. Brelsfoard CL, Mains JW, Mulligan S, Cornel A, Holeman J, Kluh S, et al. Aedes aegypti males as vehicles for insecticide delivery. Insects. 2019;2019:230.

    Google Scholar 

  18. Chen YA, Lai YT, Wu KC, Yen TY, Chen CY, Tsai KH. Using UPLC-MS/MS to evaluate the dissemination of pyriproxyfen by Aedes mosquitoes to combat cryptic larval habitats after source reduction in Kaohsiung in Southern Taiwan. Insects. 2020;11:251.

    PubMed Central  Google Scholar 

  19. Devine GJ, Perea EZ, Killeen GF, Stancil JD, Clark SJ, Morrison AC. Using adult mosquitoes to transfer insecticides to Aedes aegypti larval habitats. Proc Natl Acad Sci USA. 2009;106:11530–4.

    CAS  PubMed  PubMed Central  Google Scholar 

  20. Day JF. Mosquito oviposition behavior and vector control. Insects. 2016;7:65.

    PubMed Central  Google Scholar 

  21. Andreo V, Porcasi X, Guzman C, Lopez L, Scavuzzo CM. Spatial distribution of Aedes aegypti oviposition temporal patterns and their relationship with environment and dengue incidence. Insects. 2012;12:919.

    Google Scholar 

  22. Siriporn P, Mayura S. The effects of herbal essential oils on the oviposition-deterrent and ovicidal activities of Aedes aegypti (Linn.), Anopheles dirus (Peyton and Harrison) and Culex quinquefasciatus (Say). Trop Biomed. 2012;29:138–50.

    CAS  PubMed  Google Scholar 

  23. Seenivasagan T, Iqbal ST, Guha L. Forced egg retention and oviposition behavior of malaria, dengue and filariasis vectors to a topical repellent diethylphenylacetamide. Indian J Exp Biol. 2015;53:440–5.

    CAS  PubMed  Google Scholar 

  24. Satho T, Dieng H, Muhammad Hishamuddin IA, Salbiah BE, Abu Hassan A, Abang FB, et al. Coffee and its waste repel gravid Aedes albopictus females and inhibit the development of their embryos. Parasit Vectors. 2015;8:272.

    PubMed  PubMed Central  Google Scholar 

  25. Hoel DF, Obenauer PJ, Clark M, Smith R, Hughes TN, Larson RT, et al. Efficacy of ovitrap colors and patterns for attracting Aedes albopictus at suburban field sites in north-central Florida. J Am Mosq Control Assoc. 2011;27:245–51.

    PubMed  Google Scholar 

  26. Tsunoda T, Nguyen DT, Quynh TV. Effects of color and perforated lid on ovitrap preference of Aedes aegypti and Aedes albopictus. J Am Mosq Control Assoc. 2020;36:240–4.

    PubMed  Google Scholar 

  27. O’Gower A. The influence of the surface on opposition by Aedes albopictus (Skuse) and Aedes scutellaris katherinensis Woodhill (Diptera, Culicidae). Proc Linn Soc NS Wales. 1957a;82:285–8.

    Google Scholar 

  28. O’Gower A. The influence of the surface on oviposition by Aedes aegypti (Linn.) (Diptera, Culicidae). Proc Linn Soc NS Wales. 1957b;82:240–4.

    Google Scholar 

  29. Oower A. Environmental stimuli and the oviposition behaviour of Aedes aegypti var. queenslandis (Theobald Diptera Culicidae). Anim Behav. 1963;11:189–97.

    Google Scholar 

  30. Harrington LC, Ponlawat A, Edman JD, Scott TW, Vermeylen F. Influence of container size, location, and time of day on oviposition patterns of the dengue vector, Aedes aegypti, in Thailand. Vector-Borne Zoo Dis. 2008;8:415–23.

    CAS  Google Scholar 

  31. Garrett WD, White SA. Monomolecular organic surface films: I. Selection of optimum film-forming agents. Mosq News. 1977;37:344–50.

    CAS  Google Scholar 

  32. Dawood A-FD, Baz MM, Ibrahim MI. Influence of Aquatain™, a monomolecular surface film on surface tension for controlling the filarial vector Culex pipiens (Diptera: Culicidae). Heliyon. 2020;6:e05314.

    PubMed  PubMed Central  Google Scholar 

  33. Otremba Z. The influence of an oil-film covered sea surface on the reflection and upward transmission of light. Oceanologia. 1994;36:137–54.

    Google Scholar 

  34. Otremba Z. The impact on the reflectance in VIS of a type of crude oil film floating on the water surface. Opt Express. 2000;7:129–34.

    CAS  PubMed  Google Scholar 

  35. Speight JG. The properties of water. In: Speight JG, editor. Natural water remediation. Oxford: Butterworth-Heinemann; 2020.

  36. Mulla MS, Chaudhury FB. The effects of surface tension on pupae Culex pipiens quinquefasciatus say and Aedes aegypti (L.). Mosq News. 1968;28:187–91.

    Google Scholar 

  37. Oliva CF, Jacquet M, Gilles J, Lemperiere G, Maquart PO, Quilici S, et al. The sterile insect technique for controlling populations of Aedes albopictus (Diptera: Culicidae) on reunion island: mating vigour of sterilized males. PLoS ONE. 2012;7: e49414.

    CAS  PubMed  PubMed Central  Google Scholar 

  38. Wong J, Astete H, Morrison AC, Scott TW. Sampling considerations for designing Aedes aegypti (Diptera: Culicidae) oviposition studies in Iquitos, Peru: substrate preference, diurnal periodicity, and gonotrophic cycle length. J Med Entomol. 2011;48:45–52.

    PubMed  Google Scholar 

  39. da Costa CF, Dos Passos RA, Lima J, Roque RA, de Souza SV, Campolina TB, et al. Transovarial transmission of DENV in Aedes aegypti in the Amazon basin: a local model of xenomonitoring. Parasit Vectors. 2017;10:249.

    PubMed  PubMed Central  Google Scholar 

  40. Warikoo R, Wahab N, Kumar S. Oviposition-altering and ovicidal potentials of five essential oils against female adults of the dengue vector Aedes aegypti L. Parasitol Res. 2011;109:1125–31.

    PubMed  Google Scholar 

  41. da Silva RCS, Milet-Pinheiro P, Bezerrada da Silva PC, da Silva AG, da Silva MV, Navarro DMdAF, et al. (E)-Caryophyllene and α-Humulene: Aedes aegypti oviposition deterrents elucidated by gas chromatography-electrophysiological assay of Commiphora leptophloeos leaf oil. PLoS ONE. 2015;10:e0144586.

    PubMed  PubMed Central  Google Scholar 

  42. Andrade-Ochoa S, Sánchez-Aldana D, Chacón-Vargas KF, Rivera-Chavira BE, Sánchez-Torres LE, Camacho AD, et al. Oviposition deterrent and larvicidal and pupaecidal activity of seven essential oils and their major components against Culex quinquefasciatus Say (Diptera: Culicidae): synergism–antagonism effects. Insects. 2018;9:25.

    PubMed Central  Google Scholar 

  43. Reiter P. The action of lecithin monolayers on mosquitoes III. Studies in irrigated rice-fields in Kenya. Trop Med. 1979;74:541–57.

    Google Scholar 

  44. Reiter P, McMullen AI. The action of lecithin monolayers on mosquitoes I. General observations. Ann Trop Med Parasitol. 1978;72:163–8.

    CAS  PubMed  Google Scholar 

  45. Batra CP, Mittal PK, Adak T, Subbarao SK. Efficacy of Agnique MMF monomolecular surface film against Anopheles stephensi breeding in urban habitats in India. J Am Mosq Control Assoc. 2006;22:426–32.

    CAS  PubMed  Google Scholar 

  46. Mulla MS, Darwazeh HA, Luna LL. Monolayer films as mosquito control agents and their effects on nontarget organisms. Mosq News. 1983;43:489–96.

  47. Levy R, Chizzonite JJ, Garrett WD, Miller TW. Efficacy of the organic surface film isostearyl alcohol containing two oxyethylene groups for control of Culex and Psorophora mosquitoes: laboratory and field studies. Mosq News. 1982;41:1–11.

    Google Scholar 

  48. Nayar JK, Ali A. A review of monomolecular surface films as larvicides and pupicides of mosquitoes. J Vector Ecol. 2003;28:190–9.

    PubMed  Google Scholar 

  49. Kavran M, Pajović I, Petrić D, Ignjatović-Ćupina A, Latinović N, Jovanović M, et al. Aquatain AMF efficacy on juvenile mosquito stages in control of Culex pipiens complex and Aedes albopictus. Entomol Exp Appl. 2020;168:148–57.

    CAS  Google Scholar 

  50. Mbare O, Lindsay SW, Fillinger U. Aquatain® Mosquito Formulation (AMF) for the control of immature Anopheles gambiae sensu stricto and Anopheles arabiensis: dose-responses, persistence and sub-lethal effects. Parasit Vectors. 2014;7:438.

    PubMed  PubMed Central  Google Scholar 

  51. Dieng H, Satho T, Abang F, Miake F, Ghani IA, Latip NA, et al. Anti-oviposition activities of used sock media against a dengue vector: prospects of eco-friendly control and solutions to pollution. Environ Sci Pollut Res Int. 2017;24:21375–85.

    PubMed  Google Scholar 

  52. Farjana T, Tuno N. Effect of body size on multiple blood feeding and egg retention of Aedes aegypti (L.) and Aedes albopictus (Skuse) (Diptera: Culicidae). Med Entomol Zool. 2012;63:1–9.

    Google Scholar 

  53. Systat Software Inc. Systat 13 data. Systat for Windows: statistics. Richmond: Systat Software Inc.

  54. Reiskind MH, Zarrabi AA. Water surface area and depth determine oviposition choice in Aedes albopictus (Diptera: Culicidae). J Med Entomol. 2012;49:71–6.

    PubMed  Google Scholar 

  55. Reyes-Villanueva F, Juárez-Eguia M, Flores-Leal A. Effects of sublethal dosages of Abate® upon adult fecundity and longevity of Aedes aegypti. J Am Mosq Control Assoc. 1990;6:739–41.

    CAS  PubMed  Google Scholar 

  56. David MR, Dantas ES, Maciel-de-Freitas R, Codeço Cláudia T, Prast AE, Lourenço-de-Oliveira R. Influence of larval habitat environmental characteristics on culicidae immature abundance and body size of adult Aedes aegypti. Front Ecol Evol. 2012;9:70.

    Google Scholar 

  57. Lee SJ, Kim JH, Lee SC. Effects of oil-film layer and surfactant on the siphonal respiration and survivorship in the fourth instar larvae of Aedes togoi mosquito in laboratory conditions. Sci Rep. 2018;8:5694.

    PubMed  PubMed Central  Google Scholar 

  58. Ngrenngarmlert W, Sukkanon C, Yaicharoen R, Chareonviriyaphap T. Physical influence on larvicidal and pupicidal activity of the silicone-based monomolecular film. Acta Trop. 2016;162:239–44.

    CAS  PubMed  Google Scholar 

  59. Likura H, Takizawa H, Ozawa S, Nakagawa T, Matsui Y, Nambu H. Mosquito repellence induced by tarsal contact with hydrophobic liquids. Sci Rep. 2020;10:14480.

    Google Scholar 

  60. Chadee DD. Effects of forced egg-retention on the oviposition patterns of female Aedes aegypti (Diptera: Culicidae). Bull Entomol Res. 1997;87:649–51.

    Google Scholar 

  61. Xue RD, Ali A, Barnard DR. Effects of forced egg-retention on adult survival and reproduction following application of DEET as an oviposition deterrent. J Vector Ecol. 2005;30:45–8.

    PubMed  Google Scholar 

  62. Bibbs CS, Hahn DA, Kaufman PE, Xue RD. Sublethal effects of a vapour-active pyrethroid, transfluthrin, on Aedes aegypti and Ae. albopictus (Diptera: Culicidae) fecundity and oviposition behaviour. Parasit Vectors. 2018;11:486.

    PubMed  PubMed Central  Google Scholar 

  63. Chadee DD. The diel oviposition periodicity of Aedes aegypti (L.) (Diptera: Culicidae) in Trinidad, West Indies: effects of forced egg retention. Bull Entomol Res. 2010;100:599–603.

    CAS  PubMed  Google Scholar 

  64. Gillies MT. A review of some recent Russian publications on the technique of age determination in Anopheles. Trop Dis Bull. 1958;55:713–21.

    CAS  PubMed  Google Scholar 

  65. Elsie JG, Judson CL. Enforced egg-retention and its effect on vitellogenesis in the mosquito Aedes aegypti. J Med Entomol. 1972;9:527–30.

    Google Scholar 

  66. Magnarelli LA. Egg retention in mosquitoes (Diptera: Culicidae) and its relation to physiological age. Mosq News. 1975;35:396–9.

    Google Scholar 

  67. Bentley M, Day JF. Chemical ecology and behavioral aspects of mosquito oviposition. Annu Rev Entomol. 1989;34:401–21.

    CAS  PubMed  Google Scholar 

  68. Nakhleh J, El Moussawi L, Osta, MA. The melanization response in insect immunity. In: Ligoxygakis P, editor. Advances in insect physiology. Cambridge: Academic Press; 2017.

  69. Kim SR, Yao R, Han Q, Christensen BM, Li J. Identification and molecular characterization of a prophenoloxidase involved in Aedes aegypti chorion melanization. Insect Mol Biol. 2005;14:185–94.

    CAS  PubMed  PubMed Central  Google Scholar 

  70. Thomas P, Kenny N, Eyles D, Moreira LA, O’Neill SL, Asgari S. Infection with the wMel and wMelPop strains of Wolbachia leads to higher levels of melanization in the hemolymph of Drosophila melanogaster, Drosophila simulans and Aedes aegypti. Dev Comp Immunol. 2011;35:360–5.

    CAS  PubMed  Google Scholar 

  71. Isoe J, Koch LE, Isoe YE, Rascón AA Jr, Brown HE, Massani BB, Miesfeld RL. Identification and characterization of a mosquito-specific eggshell organizing factor in Aedes aegypti mosquitoes. PLoS Biol. 2019;17: e3000068.

    PubMed  PubMed Central  Google Scholar 

  72. Clements AN. The biology of mosquitoes. Development, nutrition and reproduction. London: Chapman and Hall; 1992.

    Google Scholar 

  73. Huang CY, Christensen BM, Chen CC. Role of dopachrome conversion enzyme in the melanization of filarial worms in mosquitoes. Insect Mol Biol. 2005;14:675–82.

    PubMed  Google Scholar 

  74. Dieng H, Boots M, Tamori N, Higashihara J, Okada T, Kato K, et al. Some technical and ecological determinants of hatchability in Aedes albopictus, a potential candidate for transposon-mediated transgenesis. J Am Mosq Control Assoc. 2006;22:382–9.

    PubMed  Google Scholar 

  75. Farnesi LC, Vargas HCM, Valle D, Rezende GL. Darker eggs of mosquitoes resist more to dry conditions: melanin enhances serosal cuticle contribution in egg resistance to desiccation in Aedes, Anopheles and Culex vectors. PLoS Negl Trop Dis. 2017;11: e0006063.

    PubMed  PubMed Central  Google Scholar 

  76. Karlson P, Sekeris CE. N acetyldopamine as sclerotizing agent of the insect cuticle. Nature. 1962;95:183–4.

    Google Scholar 

  77. Ultimate Agri-Products Pty Ltd. Aquatain independent water quality report. 2007.http://www.aquatain.com.au. Accessed 21 Nov 2021.

  78. The Public Health and Safety Organization (NSF). Certificate for use on drinking water in USA. 2008.http://www.nsf.org/Certified/PwsChemicals/Listings.asp?Company=4Q360&Standard=060&. Accessed 22 Nov 2021.

  79. Sugumaran M, Barek H. Critical analysis of melanogenic pathway in insects and higher animals. Int J Mol Sci. 2016;17:1753.

    PubMed Central  Google Scholar 

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Acknowledgements

The authors are grateful to the Disease Prevention Officers Tariq Webb and Rico Reid of the Mosquito Research and Control Unit (MRCU). The authors also thank the Chief Officer (Nellie Pouchie) and Minister Sabrina Turner, Ministry for Health and Wellness of Cayman Islands, for providing financial assistance for this internship program of MRCU.

Funding

The Ministry for Health and Wellness of the Cayman Islands supported this work.

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Authors and Affiliations

  1. Mosquito Research and Control Unit (MRCU), George Town, Cayman Islands

    Hamady Dieng, Whitney Ebanks, Zoila Ebanks & Alan Wheeler

  2. The University College of the Cayman Islands, Olympic Way, George Town, Cayman Islands

    Storm McLean & Malik Gordon

  3. The University of Liverpool, Liverpool, L69 3BX, UK

    Holly Stradling

  4. The Forensic Department, Health Services Authority, George Town, Cayman Islands

    Cole Morgan

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Contributions

HD and AW conceived and designed the study. ST, HS, CM, WME, ZE and HD performed the bioassays. HD and AW analyzed the data. HD drafted the manuscript. All authors brought essential insights and all of them read and approved the final manuscript.

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Correspondence to Hamady Dieng.

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Dieng, H., McLean, S., Stradling, H. et al. Aquatain® causes anti-oviposition, egg retention and oocyte melanization and triggers female death in Aedes aegypti. Parasites Vectors 15, 100 (2022). https://doi.org/10.1186/s13071-022-05202-0

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Parasites & Vectors

ISSN: 1756-3305

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