Odour-mediated oviposition site selection in Aedes aegypti depends on aquatic stage and density
Parasites & Vectors volume 16, Article number: 264 (2023)
Olfaction plays an important role in the selection and assessment of oviposition sites by mosquitoes. Volatile organic compounds (VOCs) associated with potential breeding sites affect the behaviour of gravid mosquitoes, with VOCs from aquatic stages of conspecific mosquitoes influencing and regulating oviposition. The purpose of this study was to conduct a systematic analysis of the behavioural response of gravid Aedes aegypti to conspecific aquatic stage-conditioned water, to identify the associated bioactive VOCs and to determine how blends of these VOCs regulate oviposition site selection and stimulate egg-laying.
Using a multi-choice olfactory oviposition assay, controlling for other sensory modalities, the responses of individual females to water conditioned with different densities of conspecific aquatic stages were assessed. The conditioned water samples from the most preferred density of each aquatic stage were subsequently compared to each other using the same oviposition assay and analysed using an analysis of variance (ANOVA) followed by a Tukey post-hoc test. Using combined gas chromatography and electroantennographic detection or mass spectrometry, bioactive VOCs from the preferred density of each aquatic stage were identified. Synthetic blends were prepared based on the identified ratios of bioactive VOCs in the aquatic stages, and then tested to determine the oviposition choice of Ae. aegypti in a dose-dependent manner, against a solvent control, using a dual-choice assay. This dataset was analysed using nominal logistic regression followed by an odds ratio comparison.
Gravid Ae. aegypti responded stage- and density-dependently to water conditioned with eggs, second- and fourth-instar larvae, and pupal exuviae, but not to water conditioned with pupae alone. Multi-choice assays demonstrated that gravid mosquitoes preferred to oviposit in water conditioned with fourth-instar larvae, over the other aquatic stage-conditioned water. Gravid Ae. aegypti were attracted, and generally stimulated, to oviposit in a dose-dependent manner to the individual identified synthetic odour blends for the different aquatic stages.
Intraspecific VOCs regulate oviposition site selection in Ae. aegypti in a stage- and density-dependent manner. We discuss the need for further studies to evaluate the identified synthetic blends to modulate the odour-mediated oviposition of Ae. aegypti under field conditions.
For mosquitoes, oviposition site selection is essential, as this decision directly regulates the growth, development and survival of the next generation, as well as population dynamics [1,2,3,4,5]. The aquatic stages of mosquitoes are limited in their movement, and thus the fate of the offspring is largely dependent on the maternal selection of oviposition sites [2, 6, 7]. While seeking oviposition sites, gravid mosquitoes must search for, and distinguish between, potential oviposition sites over multiple spatial scales to ensure the availability of nutrients for larval development and survival, and to reduce competition and offspring mortality [2, 8,9,10]. For this purpose, mosquitoes rely predominantly on olfactory cues emanating from potential oviposition sites and their surroundings [6, 9, 11]. Emanates from conspecific immature stages associated with breeding sites can act as reliable signals for females to assess the quality of an oviposition site, in terms of overcrowding and competition from con- and heterospecific aquatic stages . An increased understanding of the signals regulating conspecific oviposition site selection may lead to the development of species- and/or genera-specific attractants for vector control.
Oviposition site selection by gravid mosquitoes can be modulated by cues associated with the aquatic stages, in a species-, stage- and density-dependent manner . Gravid mosquitoes generally avoid ovipositing in breeding sites in which the risk of con- and heterospecific competition and cannibalism/predation is high [12,13,14,15,16,17,18,19]. The manner by which individual species assess oviposition sites differs in accordance with species-specific breeding site requirements [2, 6, 11, 20]. This is, therefore, dependent on the ability of gravid females to evaluate cues emanating from distinct conspecific aquatic stages, as these provide reliable signals of breeding site conditions [11, 12, 15, 18, 19]. Limitation in nutrient resources, regulated by, e.g., competition and the dynamic nature of mosquito-associated microbial communities, differentially affects oviposition site choice in a taxon-dependent manner [5, 6, 19, 21, 22]. In addition, the persistence of individual breeding sites affects mosquitoes species-specifically, often depending on the drought tolerance of the aquatic stages, with conspecific stage-associated cues providing reliable temporal information concerning, e.g., ephemeral and cyclically flooded sites [2, 6, 21]. For example, gravid yellow fever and Asian tiger mosquitoes Aedes aegypti and Aedes albopictus, respectively, preferentially select breeding sites that contain or have previously contained, late aquatic stages, which is believed to indicate the availability of larval food resources [20, 22]. The density of the conspecific aquatic stages in the breeding sites also modulates mosquito oviposition site selection, as overcrowding leads to competition while low conspecific densities increase the risk of predation, with optimal densities being species-dependent [12, 15, 17, 18, 23,24,25]. While a limited number of behaviourally active volatile organic compounds (VOCs) have been identified associated with conspecific aquatic stages, there is a further need for a systematic cross-disciplinary chemical ecological analysis to identify intraspecific signals regulating oviposition site selection and egg laying in mosquitoes .
This study aimed at exploring the stage- and density-dependent behavioural response of the yellow fever mosquito Ae. aegypti during oviposition site selection and egg-laying, as well as identifying the natural bioactive VOCs associated with water conditioned with aquatic stages, regulating this choice. Synthetic blends of these bioactive VOCs were evaluated for their ability to manipulate the oviposition response of gravid Ae. aegypti. Understanding oviposition in mosquitoes, and the bioactive VOCs involved, will assist in enhancing existing vector surveillance and control programmes by targeting gravid mosquitoes to reduce vector populations and the burden of disease transmission.
Aedes aegypti (Rockefeller) eggs, laid on filter paper (90 mm diameter; Ahlstrom, Munksjö, Finland), were placed in 3-l plastic rearing trays (L: 24.5 × W: 18.5 × H: 7.5 cm; Emballator Lagan AB, Ljungby, Sweden) filled with 1 l distilled water. Larvae were fed daily with TetraMin® fish food (Tetra GmbH, Melle, Germany). The pupae were collected in 30-ml containers (Essentra Components, Malmö, Sweden) kept in a BugDorm-1 cage (L: 30 × W: 30 × H: 30 cm; MegaView Science, Taichung, Taiwan) for adult emergence. Adults were maintained at 27 ± 1 °C, 65 ± 5% relative humidity, and at a 12:12 h light–dark cycle, with ad libitum access to a 10% sucrose solution. For colony maintenance and experiments, adults 5–7 days post-emergence (dpe) were provided with sheep blood (Håtunalab, Bro, Sweden) for 2 h using a collagen membrane through a Hemotek membrane feeding system (Hemotek Ltd., Blackburn, UK) at 37 °C. Fully engorged females were used in the oviposition experiments, five days after blood meal ingestion (10–12 dpe).
Conditioning water with aquatic stages of Aedes aegypti
Water was conditioned with eggs, second-instar larvae, fourth-instar larvae, pupae or pupal casings of Ae. aegypti. To produce the egg-conditioned water (ECW), filter papers containing c. 250, 500, 1000 and 2000 eggs were collected and incubated at −20 °C for 30 min to prevent hatching. This treatment is unlikely to have damaged the chorion or outer egg casing , and thus unlikely to affect the VOCs released. Individual filter papers, with or without eggs, were then placed in rearing trays containing 1 l distilled water for 22 ± 2 h. To obtain the larvae-conditioned water (LCW), first-instar larvae were transferred to rearing trays (see above) containing one of four densities (c. 50, 150, 300 and 600 larvae l−1), and reared to second instar or fourth instar without changing the water prior to subsequent assays. Throughout its development, each larva was fed c. 10 mg of TetraMin fish food, with first- to early third-instar larvae provided with 0.6 mg of food larva per day, and late third- and fourth-instar larvae provided with 2 mg of food larva per day. As a control, distilled water was treated with equivalent amounts of fish food and under the same conditions, with food particles sieved out daily prior to the next allotment of fish food to reflect the consumption of food by the larvae. To generate the water conditioned with pupae and their exuviae, two groups of pupae were collected. The pupae, at densities of either c. 50, 100, 150 and 300 or 6, 12, 24 and 48, were rinsed with distilled water to remove any extraneous particles and then transferred to rearing trays containing 1 l of distilled water. The first group of pupae were kept for 22 ± 2 h to produce the pupae-conditioned water (PCW). The second group of pupae were retained until all adults emerged (3 nights), and only the exuviae remained in the distilled water, after which the exuviae-conditioned water (XCW) was obtained. As controls, 1 l of distilled water was kept without pupae or pupal exuviae over the same time period under the same conditions. The conditioned water was then strained through nylon mesh and a folded filter paper (18.5 cm; Whatman International Ltd., Maidstone, England), and used immediately in subsequent assays.
Multi-choice oviposition assay
To characterize the density-dependent effect of odours emanating from water conditioned with aquatic stages on oviposition site selection and egg laying by gravid Ae. aegypti, multi-choice oviposition assays were performed (Additional file 1: Fig. S1a). The conditioned water (40 ml of test or control) was added into the bottom section of an artificial oviposition site consisting of a blue plastic cup (250 ml; Duni, Malmö, Sweden), within which a second transparent cup (120 ml; ÖoB, Lund, Sweden), with six 2.5-mm-diameter perforations in the bottom, was placed in order to exclude input from sensory modalities other than olfaction (Additional file 1: Fig. S1b). A third cup (30 ml), containing distilled water and a filter paper, was placed inside the second cup (Additional file 1: Fig. S1b). The filter paper served as the oviposition substrate. Artificial oviposition sites containing the water conditioned with different densities of each aquatic stage and a distilled water control were placed in a BugDorm-1 cage. The treatments and control were randomly designated among the five artificial oviposition sites within the cage, one artificial oviposition site in each corner and one in the middle of the cage (Additional file 1: Fig. S1a). Five days after blood-feeding, an individual gravid mosquito (10–12 dpe) was released into each cage 2 h prior to scotophase, and provided ad libitum access to 10% sucrose. The placement of the sucrose dispensers alternated between the left and right sides of the cages, and had no effect on oviposition choice. The bioassays were kept under similar climate conditions for 48 h, as described above, after which the eggs laid in each artificial oviposition site were counted.
Solid-phase microextraction headspace collections
Solid-phase microextraction (SPME) divinylbenzene/carboxen/polydimethylsiloxane Supelco StableFlex™ fibres (50/30 µm, 24 ga, 2 cm; Sigma-Aldrich, Stockholm, Sweden) were conditioned at 225 °C for 30 min using a gas chromatograph (GC; Agilent Technologies 6890, Santa Clara, CA, USA) prior to headspace collections. The glassware used for headspace collections was cleaned and placed at 250 °C for 8 h prior to use. Either the conspecific aquatic stage-conditioned water eliciting the highest oviposition response in the multi-choice assays (400 ml) or the control water (400 ml) was poured into 1 l glass bottles (VWR, Stockholm, Sweden). The water used for these odour collections was conditioned to match that of the conditioned water used in the behavioural experiments. Thereafter, sodium chloride (NaCl; ≥ 99%, Sigma-Aldrich), was dissolved into each to enhance the emission of volatiles following modified protocols of Lindh et al.  and Mozūraitis et al. . Three concentrations of NaCl (150, 225 and 255 mg ml−1) were tested, from which it was determined that 255 mg ml−1 elicited the highest abundance of VOCs trapped on the SPME fibre from the conditioned water. The water was then incubated at room temperature for c. 5 min. The PCW was omitted due to the lack of a density-dependent oviposition response (Additional file 1: Fig. S2). The clean SPME fibre was introduced into a small hole (1.4 mm diameter) drilled in the polypropylene lid of the glass bottle containing the samples to collect the headspace for 17 h.
Combined gas chromatography and electroantennographic detection
Antennal responses of 5-day post-blood-fed (10–12 dpe) Ae. aegypti to VOCs contained within the headspace collected on the SPME fibre of each of the aquatic stage-conditioned water were determined using combined gas chromatography (GC), flame ionization detection (FID) and electroantennographic detection (EAD) analyses. The GC (Agilent Technologies 6890) was equipped with an HP-5 column (30 m length × 0.25 mm inner diameter [i.d.] × 0.25 µm film thickness) and an effluent splitter between the column and the detectors. Hydrogen was used as the carrier gas at a linear flow rate of 45 cm s−1. The VOCs adsorbed onto the SPME fibres were injected into the GC in splitless mode for 1 min at 225 °C and thermally desorbed in the inlet. The GC oven temperature was programmed from 50 °C (hold for 1 min), increased at a rate of 8 °C min−1 to 275 °C (10 min hold). At the GC effluent splitter, nitrogen was added and the gas flow split between the FID and the EAD in a 1:1 volume four-way cross-splitter (Gerstel, Mülheim, Germany). The GC effluent moving towards the EAD passed through a Gerstel Olfactory Detector Port (ODP)-2 transfer line (Gerstel) that tracked the GC oven temperature before it was delivered into a glass tube (10 cm × 8 mm), where it was mixed with charcoal-filtered humidified air (1.5 l min−1). The antennal preparation was positioned 0.5 cm away from the outlet of the glass tube.
For the EAD analysis, a female mosquito was cold anesthetized prior to mounting the excised head on a reference electrode, which was inserted through the foramen. The cut, distal flagellomere of the antenna was connected to the recording electrode. Both electrodes were made from pulled glass microcapillaries, filled with Beadle–Ephrussi Ringer solution  and placed over chlorinated silver wires in the electrode holders. The recording electrode was attached to a pre-amplifier (1×), then to a high-impedance direct current (DC) amplifier interface (IDAC-2 Ockenfels Syntech GmbH, Buchenbach, Germany) and finally to a personal computer (PC) for visualization and storage. Three to five stable recordings were performed for the headspace collected from the water conditioned with each aquatic stage. The data were analysed using GC-EAD software (v.1.2.3, Ockenfels Syntech GmbH).
The SPME samples from each of the aquatic stage-conditioned water and the corresponding controls were injected into a combined GC (6890, Agilent Technologies) and mass spectrometer (MS, 5975, Agilent Technologies) operated in the electron ionization mode at 70 eV. The GC–MS unit was equipped with the same type of fused silica capillary HP-5 column (60 m length × 0.25 mm i.d. × 0.25 µm film thickness) as the GC–EAD. Helium was used as the carrier gas at a linear flow rate of 34 cm s−1. The same temperature programme was used for both the GC–MS and the GC–EAD analyses. A total of three to five SPME samples, collected from the water conditioned with each of the aquatic stages and control, were injected into the GC–MS. All physiologically active VOCs, which were determined using GC–EAD analysis, were identified using linear retention times (Kovats index) and mass spectra in comparison with the National Institute of Standards and Technology (NIST) 17 library, and subsequently confirmed with authentic standards (Table 1). The relative abundance of the bioactive VOCs in each of the extracts was approximated by comparing the areas of each total ion chromatogram. The approximate relative abundance of each compound was then used to formulate the synthetic blends. The composition and ratio of, as well as the physiological response to, the compounds used in the synthetic blends were confirmed using GC–MS and GC–EAD, respectively. The purity of the commercial compounds was confirmed by injection on the GC–MS (Table 1).
Dual-choice oviposition bioassay with synthetic blends
To determine the behavioural preference of gravid Ae. aegypti to the identified synthetic blends from the water conditioned with the different conspecific aquatic stages, a dose-dependent analysis was performed in a dual-choice oviposition assay. The artificial oviposition sites, containing either the treatment or the control, were placed in opposite corners of a BugDorm-1 cage, c. 8 cm from each cage wall. Each dilution of an individual synthetic blend (6 ml) was tested against a solvent control (6 ml hexane). Both the blend and the control were delivered from wick dispensers , constructed of a 12-ml vial (Genetec, Stockholm, Sweden) with a perforated lid (2-mm diameter hole) and a wick. The wick was made from Teflon tubing (75 mm length × 1.68 mm i.d. × 0.30 mm wall thickness), with a piece of unbleached cotton string inserted . The wick dispensers allowed for the control of the release rate and ratio of the VOCs in the blend during the bioassay . Each wick dispenser was then placed in a 250 ml glass wash bottle (VWR). Charcoal-filtered air was passed through the glass wash bottles, via Teflon tubing (6 mm outer diameter [o.d.]), using an air pump (model V-20; Guangdong Hailea Group Co., Ltd., Guangdong, China), into two 12-channel flow meters (Kytola Instruments, Muurame, Finland), in which the flow rate was adjusted to 0.1 l min−1. Teflon tubing connected the flow meters to the artificial oviposition sites (Additional file 1: Fig. S3) . Individual 5-day post-blood-fed Ae. aegypti were introduced into each of the 12 BugDorm-1 cages containing the artificial oviposition sites, 2 h prior to scotophase. Females were offered ad libitum access to 10% sucrose during the bioassay (19 ± 1 h). Subsequently, the number of eggs laid in the treatment and the control was counted and oviposition choice indices were calculated: C/(C + T) and T/(T + C), in which C is the number of eggs laid in the control and T is the number of eggs laid in the treatment. Dual-choice assays with solvent-filled wick dispensers on both sides determined that there was no positional bias in the egg-laying choice of the gravid mosquitoes (Additional file 1: Fig. S4) . Three or four replicates, each containing 12 mosquitoes, were performed.
The Shapiro–Wilk test was performed to test for a normal distribution of eggs laid by each female, which determined that all the datasets failed the assumption of normality (JMP Pro version 16, SAS Institute Inc., Cary, NC, 1989–2021). The datasets for the multi-choice assays across different densities of each aquatic stage, and across the most preferred densities of a conspecific aquatic stage, were compared using the average total number of eggs laid per female by analysis of variance (ANOVA) followed by a Tukey post-hoc test. For the multi-choice assays, the artificial oviposition sites were rotated through each of the five positions, to minimize any location bias. Following the ECW and XCW experiments, the data were analysed using a general linear model (JMP Pro version 16), determining that there was no positional bias in the egg-laying response of gravid Ae. aegypti to these treatments, ECW (χ2 = 12.84, df = 8, P = 0.12) and XCW (χ2 = 9.71, df = 8, P = 0.29). For dual-choice assays, a binary logistic regression followed by odds ratio comparison was used to test for oviposition site preference, while, an ANOVA followed by a Tukey post-hoc test was used to assess egg stimulation in response to both treatments and controls (JMP Pro version 16). The egg-laying response was the dependent variable determined by the number of gravid females in the oviposition bioassay, and dose was the independent fixed effect.
Water conditioned with aquatic stages affects oviposition
To assess the effect of water conditioned with different densities of aquatic stages of Ae. aegypti on the behavioural response of gravid mosquitoes, a series of multi-choice oviposition assays were conducted (Fig. 1a–d; Additional file 1: Figs. S1 and S2). Gravid mosquitoes demonstrated an overall density-dependent response to water conditioned with each aquatic stage compared to the control, as assessed using an ANOVA followed by a Tukey post-hoc test, for ECW (F = 2.72, P = 0.029); second-instar LCW (F = 3.89, P = 0.0042); fourth-instar LCW (F = 2.90, P = 0.021); and XCW (F = 2.76, P = 0.027); but not for PCW (F = 0.61, P = 0.66; Fig. 1a–d; Additional file 1: Fig. S2). In all experiments, gravid mosquitoes demonstrated a preference for conditioned water that had contained an intermediate density of the aquatic stages (Fig. 1a–d), with the exception of PCW, for which there was no preference for any density (Additional file 1: Fig. S2). When gravid mosquitoes were given the choice of the most preferred density of ECW, second-instar and fourth-instar LCW, PCW, and XCW in a subsequent multi-choice oviposition assay, individual gravid mosquitoes preferred to lay significantly more eggs in water conditioned with fourth-instar larvae (F = 7.46, P < 0.0001; Fig. 2).
Bioactive compounds identified in water conditioned with aquatic stages
While combined GC–EAD and GC–MS analyses identified nine bioactive VOCs associated with the ECW extracts, only four (2,4-dimethylhept-1-ene, 2,6-dimethyl-7-octen-2-ol, camphor and decanal) were present in this treatment and not in the control, and thus are considered egg-associated compounds (Fig. 1e). Similarly, of the six and 11 bioactive VOCs from the second- and fourth-instar LCW, five (4-cyanocyclohexene, (E)-2-octenal, nonanal, decanal and 4-(2-methylbutan-2-yl)phenol) and eight (2,4-dimethylhept-1-ene, (E)-2-heptanal, nonanal, camphor, (E)-2-nonenal, (E)-2-decenal and 4-(2-methylbutan-2-yl)phenol, and an unidentified branched C12-alkane) were found in these treatments and not in their controls (Fig. 1f, g). From the XCW samples, nine VOCs elicited a response from the antennae, three of which (4-cyanocyclohexene, 2,6-dimethyl-7-octen-2-ol and nonanal) were present in this treatment and not in the associated control (Fig. 1h). While n-heneicosane, a previously identified putative oviposition pheromone component in Ae. aegypti larvae [32, 33] was specifically sought for in each of the SPME collections, none was identified in the GC–MS analysis.
Synthetic odour blends elicit oviposition in Ae. aegypti
To assess whether synthetic odour blends, designed based on the bioactive VOCs identified to be associated with the aquatic stages of Ae. aegypti, elicit attraction and stimulation of oviposition, these were evaluated in a dual-choice assay and compared with a solvent control (hexane) (Additional file 1: Fig. S3). The synthetic blends were prepared to mimic the identified ratio of bioactive VOCs: eggs (2,4-dimethylhept-1-ene: 2,6-dimethyl-7-octen-2-ol: camphor: decanal, 6:1:17:1); second instar (4-cyanocyclohexene: (E)-2-octenal: nonanal: decanal: 4-(2-methylbutan-2-yl)phenol, 1:7:9:5:17); fourth instar (2,4-dimethylhept-1-ene: (E)-2-heptanal: nonanal: camphor: (E)-2-nonenal: (E)-2-decenal: 4-(2-methylbutan-2-yl)phenol, 11:9:3:48:1:9:20); and pupal exuviae (4-cyanocyclohexene: 2,6-dimethyl-7-octen-2-ol: nonanal, 1:6:4), respectively. The four blends were diluted in hexane and assayed at different doses against a solvent control (hexane) (Fig. 3a–d). Gravid Ae. aegypti were attracted to oviposit in a dose-dependent manner in response to each of the four synthetic blends: eggs (χ2 = 12.09, df = 3, P = 0.0071); second instars (χ2 = 15.22, df = 3, P = 0.0016); fourth instars (χ2 = 6.79, df = 3, P = 0.079); and pupal exuviae (χ2 = 11.11, df = 3, P = 0.011) (Fig. 3a–d). Moreover, the synthetic blends significantly stimulated the gravid Ae. aegypti to lay eggs dose-dependently, except in response to that of the second instars: eggs (F = 3.39, P = 0.020); second instar (F = 1.22, P = 0.30); fourth instar (F = 4.90, P = 0.0030); and pupae exuviae (F = 3.13, P = 0.027) (Fig. 3e–h). While a higher overall number of eggs were laid in response to the synthetic odour blends based on the VOCs identified associated with eggs and fourth-instar LCW (Fig. 3e, g), the eggs were laid differentially, with those laid in response to the egg-based odour blend being predominantly placed in the treatment site, and those laid in response to the fourth-instar-based odour blend being predominantly laid in the control site (Fig. 3e, g).
Volatiles associated with conspecific aquatic stages differentially attract mosquitoes to oviposition sites and stimulate egg laying [this study, 11, 12, 15, 17, 18, 20, 24, 34–40]. In this study, gravid Ae. aegypti were preferentially attracted to oviposit in response to the VOCs emanating from water conditioned with late-stage larvae [11, 20, 22], which likely signals a productive breeding site and reduced competition for resources between the existing, soon to pupate, larvae and the new generation [6, 20, 41, 42]. Furthermore, the density of the conspecific aquatic stages affected oviposition site choice, with gravid mosquitoes laying fewer eggs, and even avoiding ovipositing, on the treated sites when the odours of these sites indicated high densities of conspecific competitors [this study, 12, 15, 17, 18, 24, 25, 41, 43]. Both the aquatic stage and odour release rate significantly affected the manner in which females were stimulated to oviposit in either the treated or controlled sites. Our findings indicate that gravid mosquitoes rely on the detection of aquatic stage-specific VOC blends for the identification and discrimination among potential oviposition sites to provide a reliable signal of the suitability of a potential breeding site for their offspring [24, 39]. This differential preference for a specific conspecific aquatic stage, and its volatiles, may have a direct effect on the population dynamics of Ae. aegypti, and provide a potential route by which to manipulate vector behaviour.
The presence of conspecific aquatic stages in a breeding site, currently or in the recent past, influences and mediates the oviposition site selection and egg-laying decision of gravid mosquitoes [this study, 11, 12, 15, 17, 18, 20, 24, 34–40, 44]. The behavioural responses of gravid mosquitoes to these sites are species- and taxon-specific [34, 36, 38, 41, 44]. For example, gravid Ae. aegypti preferentially oviposit in water conditioned with late-stage larvae [this study, 20], whereas Anopheles coluzzii preferentially lay eggs in breeding sites containing first-instar larvae . This indicates that the odour profile of breeding sites changes depending on the developmental stage of conspecifics, as demonstrated in this study for Ae. aegypti, and that of Schoelitsz et al.  for An. coluzzii.
The ecological rationale for the observed taxon-specific strategies of gravid mosquitoes to use cues from particular conspecific aquatic stages as indicators of the suitability of a potential breeding site for their offspring is based on species-related differences in the ability of their offspring to withstand the changing biotic (e.g., food resources, competition) and abiotic (e.g., water availability, dissolved oxygen, salinity) conditions in the breeding sites [2, 5, 19, 20, 34, 36, 38, 41, 44,45,46]. Aedes aegypti selects breeding sites which contain/contained late-stage larvae for oviposition, which may at first seem counter-intuitive, as by the time that larvae reach the fourth instar there is the risk that these will have consumed the bulk of the resources in the restricted, local environment, and may compete with newly hatched larvae for the limited resources contained within [20, 47]. However, late-stage larvae will soon transition to the non-feeding pupal stage, thereby reducing the risk of conspecific competition with newly hatched larvae, reflecting the oviposition preference of Ae. aegypti under natural and laboratory conditions [this study, 20]. The lack of attraction of the gravid mosquitoes to the conditioned water associated with the pupal stage, as the pupae do not produce the volatile signals attracting the gravid females [this study], reflects the inability of the pupae to excrete and thereby to affect the microbiota and uric acid in the environment [48, 49]. Upon adult emergence, on the other hand, the meconium harboured within the pupa is egested, releasing the gut microbiota and other urate-based wastes into the breeding site . Moreover, infested breeding containers typically contain single cohorts of aquatic stages developing in synchrony , demonstrating that gravid mosquitoes only recolonize breeding sites in the presence of conspecific eggs, to which gravid mosquitoes are stimulated to lay larger clutches of eggs, or late aquatic stages [this study, 20], to further reduce competition for their offspring. Indirect effects related to the development of the aquatic stages of Ae. aegypti may also contribute to oviposition site preference. Breeding sites showing signs of high levels of microbial growth, specifically microbes inoculated during oviposition [51,52,53,54], and associated detritus [55,56,57] that have accumulated during conspecific larval development, provide a rich, abundant larval food source, which reduces the potential competition between established and newly hatched larvae . Gravid mosquitoes ovipositing in temporary waters, such as Ae. aegypti, may also indirectly use abiotic factors to assess potential oviposition sites, as cannibalism increases with the increasing numbers of interactions between stages as density increases due to spatial limitation, rather than due to food restriction [14, 59].
Gravid mosquitoes respond in a density-dependent manner to water that contains, or has contained, conspecific aquatic stages [this study, 12, 15, 17, 18, 24, 60]. In our study, gravid Ae. aegypti laid fewer eggs in response to water conditioned with high densities of conspecific eggs, larvae and pupal exuviae, supporting the hypothesis that laying the majority of eggs in water with low densities of conspecific aquatic stages will enhance progeny growth, development and the probability of survival, as a result of reduced competition [23, 25, 61]. In contrast, high larval densities generate competition for food resources, which affects the hatching rate and larval development, as well as adult size and survival rate [23, 25, 61, 62]. While in other mosquito species, larvae that are overcrowded, and/or starved, emit deterrent VOCs, which negatively affect the oviposition behavioural response [15, 24, 43], such VOCs have yet to be demonstrated for Ae. aegypti. Together, these density-related factors affect the fitness of gravid mosquitoes, which in turn affects the vectorial capacity [61, 63,64,65]. The assessment of the factors associated with the stage and density of immature conspecifics by gravid mosquitoes can be in large part attributed to the quality and quantity of the VOCs emanating from the potential breeding sites.
Available data indicate that mosquito taxa use distinct blends of VOCs to mediate oviposition site selection and egg-laying behaviour in a species-dependent manner [this study, 11, 31]. While mosquitoes mainly respond to species-specific VOCs, gravid females make use of signature VOCs from breeding sites, particularly select straight-chain aldehydes, monoterpenes, and straight-chain fatty acids and esters, that are commonly detected across mosquito taxa [this study, 11 and references therein, 34, 35, 66–68]. The straight-chain aldehydes [(E)-2-heptanal, (E)-2-octenal, nonanal, (E)-2-nonenal, decanal, (E)-2-decenal] and monoterpenes (2,6-dimethyl-7-octen-2-ol, camphor) identified in this study have previously been demonstrated to be emitted by multiple resources used by mosquitoes to locate floral nectar [69,70,71], host [71, 72] and oviposition site sources [11, 73], reflecting chemical parsimony, suggesting that mosquitoes are under a strong adaptative pressure to make use of the same VOCs as signals to identify various resources . In addition, these and other parsimonious VOCs, detected and used by gravid mosquitoes to locate species-dependent oviposition sites [6, 11], emanate from diverse resources, including conspecific stages , food resources [6, 75, 76], fermenting vegetation  and living vegetation associated with breeding sites [78,79,80,81]. For example, nonanal, decanal and camphor have been identified from several of the conspecific developmental stages of Ae. aegypti [this study, 45], but also from infusions of vegetation and grass pollen used by Culex quinquefasciatus and Anopheles arabiensis larvae as food sources, respectively [75,76,77, 82]. In addition, (E)-2-decenal has been reported from chicken faeces, which attracts Culex mosquitoes to preferred oviposition sites [73, 83]. Moreover, straight-chain fatty acids and esters associated with the aquatic stages of mosquitoes appear to be detected across the culicines, and play a role in oviposition site selection [34, 35, 66,67,68, 84]. While several straight-chain fatty acids and esters have been previously identified from the conspecific aquatic stages of Ae. aegypti, none were identified in this study. Moreover, the putative larval pheromone component, n-heneicosane [32, 33], was not identified from the larvae-conditioned water in this study, possibly due to the mostly insoluble nature of alkanes in water. The other compounds identified in this study are structurally diverse and have not previously been associated with oviposition sites. Evidence strongly suggests that gravid Ae. aegypti do not detect these VOCs singly, but rather as blends, or chemical codes, which enable them to discriminate among potential sites to lay their eggs.
The combined chemical and electrophysiological analyses of the stage-specific conditioned water extracts demonstrated partially overlapping, yet distinct, VOC blends that provide the basis for gravid Ae. aegypti to discriminate and select among potential breeding sites. In previous studies, single VOCs, identified from the chemical analyses of breeding sites, were tested in behavioural assays without prior experiments supporting their physiological activity. Here, we present a workflow that demonstrates the importance of combinatorial coding of VOCs by mosquitoes for oviposition site selection. This coding strategy is not restricted to conspecific signalling, but has also been demonstrated in An. arabiensis in relation to oviposition site selection among vegetative resources [75, 76, 79, 85]. An increased understanding of the chemical codes underlying oviposition site selection may lead to the development of novel odour lures used for vector control and surveillance [11, 73].
Gravid Ae. aegypti use conspecific stage- and density-dependent cues to identify potential oviposition sites. The volatile profile of oviposition sites conditioned with conspecific aquatic stages changes throughout developmental time, in terms of the quality of the VOCs emitted, providing gravid mosquitoes a means by which to discriminate among oviposition sites, as well as cues for egg stimulation. The identified stage-specific synthetic odour blends regulating oviposition site selection in Ae. aegypti may be good candidates for the development of lures to be used in integrated vector control programmes. Future research will optimize and formulate synthetic lures, and subsequently investigate the combining of select blends with, e.g., the In2Care mosquito traps , to assess whether these will improve the efficacy of attract-and-kill mosquito control devices.
Availability of data and materials
All data generated or analysed during this study are included in this published article and its supplementary information files.
Flame ionization detector
Gas chromatography–mass spectrophotometry
Volatile organic compounds
Blaustein L. Oviposition site selection in response to risk of predation: evidence from aquatic habitats and consequences for population dynamics and community structure. In: Wasser SP, editor. Evolutionary theory and processes: modern perspectives: papers in honour of Eviatar Nevo. Dordrecht: Springer; 1999. p. 441–56.
Day JF. Mosquito oviposition behavior and vector control. Insects. 2016;7:65.
Kershenbaum A, Spencer M, Blaustein L, Cohen JE. Modelling evolutionarily stable strategies in oviposition site selection, with varying risks of predation and intraspecific competition. Evol Ecol. 2012;26:955–74.
Ndenga BA, Simbauni JA, Mbugi JP, Githeko AK, Fillinger U. Productivity of malaria vectors from different habitat types in the western Kenya highlands. PLoS ONE. 2011;6:e19473.
Yoshioka M, Couret J, Kim F, McMillan J, Burkot TR, Dotson EM, et al. Diet and density dependent competition affect larval performance and oviposition site selection in the mosquito species Aedes albopictus (Diptera: Culicidae). Parasit Vectors. 2012;5:225.
Bentley MD, Day JF. Chemical ecology and behavioral aspects of mosquito oviposition. Annu Rev Entomol. 1989;34:401–21.
Kohandani F, Le Goff GJ, Hance T. Does insect mother know under what conditions it will make their offspring live. Insect Sci. 2017;24:141–9.
Alcalay Y, Tsurim I, Ovadia O. Multi-scale oviposition site selection in two mosquito species. Ecol Entomol. 2019;44:347–56.
Herrera-Varela M, Lindh J, Lindsay SW, Fillinger U. Habitat discrimination by gravid Anopheles gambiae sensu lato a push-pull system. Malar J. 2014;13:133.
Kebede A, McCann JC, Kiszewski AE, Ye-Ebiyo Y. New evidence of the effects of agro-ecologic change on malaria transmission. Am J Trop Med Hyg. 2005;73:676–80.
Khan Z, Ignell R, Hill SR. Chapter 14: Odour mediated oviposition site selection by mosquitoes. In: Ignell R, Lazzari CR, Lorenzo MG, Hill SR, editors. Sensory ecology of disease vectors. Wageningen: Wageningen Academic Publishers; 2022. p. 373–416.
Gonzalez PV, Gonzalez Audino PA, Masuh HM. Oviposition behavior in Aedes aegypti and Aedes albopictus (Diptera: Culicidae) in response to the presence of heterospecific and conspecific larvae. J Med Entomol. 2015;53:268–72.
Huang J, Miller JR, Walker ED. Cannibalism of egg and neonate larvae by late stage conspecifics of Anopheles gambiae (Diptera: Culicidae): implications for ovipositional studies. J Med Entomol. 2018;55:801–7.
Mastrantonio V, Crasta G, Puggioli A, Bellini R, Urbanelli S, Porretta D. Cannibalism in temporary waters: simulations and laboratory experiments revealed the role of spatial shape in the mosquito Aedes albopictus. PLoS ONE. 2018;13:e0198194.
Mwingira VS, Spitzen J, Mboera Leonard EG, Torres-Estrada JL, Takken W. The influence of larval stage and density on oviposition site-selection behavior of the Afrotropical malaria mosquito Anopheles coluzzii (Diptera: Culicidae). J Med Entomol. 2020;57:657–66.
Sherratt TN, Church SC. Ovipositional preferences and larval cannibalism in the Neotropical mosquito Trichoprosopon digitatum (Diptera: Culicidae). Anim Behav. 1994;48:645–52.
Sumba LA, Ogbunugafor CB, Deng AL, Hassanali A. Regulation of oviposition in Anopheles gambiae s.s: role of inter- and intra-specific signals. J Chem Ecol. 2008;34:1430–6.
Zahiri N, Rau ME, Lewis DJ. Oviposition attraction and repellency of Aedes aegypti (Diptera: Culicidae) to waters from conspecific larvae subjected to crowding, confinement, starvation, or infection. J Med Entomol. 1998;35:782–7.
Xia S. Laboratory oviposition choice of Aedes aegypti (Diptera: Culicidae) from Kenya and Gabon: effects of conspecific larvae, salinity, shading, and microbiome. J Med Entomol. 2021;58:1021–9.
Wong J, Stoddard ST, Astete H, Morrison AC, Scott TW. Oviposition site selection by the dengue vector Aedes aegypti and its implications for dengue control. PLoS Negl Trop Dis. 2011;5:e1015.
Mokany A, Shine R. Oviposition site selection by mosquitoes is affected by cues from conspecific larvae and anuran tadpoles. Austral Ecol. 2003;28:33–7.
Marques CC, Miranda C. Effect of larval, pupal, and egg extracts on the oviposition behavior of female Aedes (s) albopictus (Skuse). Rev Saude Publica. 1992;26:269–71.
Yadav R, Tyagi V, Sharma AK, Tikar SN, Sukumaran D, Veer V. Overcrowding effects on larval development of four mosquito species Aedes albopictus, Aedes aegypti Culex quinquefasciatus and Anopheles stephensi. IJRSZ. 2017;3:1–10.
Suh E, Choe D-H, Saveer AM, Zwiebel LJ. Suboptimal larval habitats modulate oviposition of the malaria vector mosquito Anopheles coluzzii. PLoS ONE. 2016;11:e0149800.
Wada Y. Effect of larval density on the development of Aedes aegypti (L.) and the size of adults. Quaest Entomol. 1965;1:4.
Kramer IM, Kreß A, Klingelhöfer D, Scherer C, Phuyal P, Kuch U, et al. Does winter cold really limit the dengue vector Aedes aegypti in Europe? Parasit Vectors. 2020;13:178.
Lindh JM, Okal MN, Herrera-Varela M, Borg-Karlson A-K, Torto B, Lindsay SW, et al. Discovery of an oviposition attractant for gravid malaria vectors of the Anopheles gambiae species complex. Malar J. 2015;14:119.
Mozuraitis R, Buda V, Borg-Karlson A-K. Optimization of solid-phase microextraction sampling for analysis of volatile compounds emitted from oestrous urine of mares. Z Naturforsch C. 2010;65c:127–33.
Ephrussi B, Beadle GW. A technique of transplantation for Drosophila. Am Nat. 1936;70:218–25.
Karlsson MF, Proffit M, Birgersson G. Host-plant location by the Guatemalan potato moth Tecia solanivora is assisted by floral volatiles. Chemoecology. 2017;27:187–98.
Mosquera KD, Khan Z, Wondwosen B, Alsanius B, Hill SR, Ignell R, et al. Odor-mediated response of gravid Aedes aegypti to mosquito-associated symbiotic bacteria. Acta Trop. 2023;237:106730.
Mendki MJ, Ganesan K, Shri P, Suryanarayana MV, Malhotra RC, Rao KM, et al. Heneicosane: an oviposition-attractant pheromone of larval origin in Aedes aegypti mosquito. Curr Sci. 2000;78:1295–6.
Seenivasagan T, Sharma KR, Sekhar K, Ganesan K, Prakash S, Vijayaraghavan R. Electroantennogram, flight orientation, and oviposition responses of Aedes aegypti to the oviposition pheromone n-heneicosane. Parasitol Res. 2009;104:827–33.
Boullis A, Mulatier M, Delannay C, Héry L, Verheggen F, Vega-Rua A. Behavioural and antennal responses of Aedes aegypti (L.) (Diptera: Culicidae) gravid females to chemical cues from conspecific larvae. PLoS ONE. 2021;16:e0247657.
Ganesan K, Mendki MJ, Suryanarayana MVS, Shri P, Malhotra RC. Studies of Aedes aegypti (Diptera: Culicidae) ovipositional responses to newly identified semiochemicals from conspecific eggs. Aust J Entomol. 2006;45:75–80.
Gonzalez PV, Gonzalez Audino PA, Masuh HM. Electrophysiological and behavioural response of Aedes albopictus to n-heinecosane, an ovipositional pheromone of Aedes aegypti. Entomol Exp Appl. 2014;151:191–7.
Laurence BR, Pickett JA. Erythro-6-acetoxy-5-hexadecanolide, the major component of a mosquito oviposition attractant pheromone. J Chem Soc Chem Commun. 1982. https://doi.org/10.1039/c39820000059.
Mwingira VS, Mboera LEG, Takken W. Synergism between nonane and emanations from soil as cues in oviposition-site selection of natural populations of Anopheles gambiae and Culex quinquefasciatus. Malar J. 2021;20:52.
Schoelitsz B, Mwingira V, Mboera LEG, Beijleveld H, Koenraadt CJM, Spitzen J, et al. Chemical mediation of oviposition by Anopheles mosquitoes: a push-pull system driven by volatiles associated with larval stages. J Chem Ecol. 2020;46:397–409.
Soman RS, Reuben R. Studies on the preference shown by ovipositing females of Aedes aegypti for water containing immature stages of the same species. J Med Entomol. 1970;7:485–9.
Dhileepan K. Physical factors and chemical cues in the oviposition behavior of arboviral vectors Culex annulirostris and Culex molestus (Diptera: Culicidae). Environ Entomol. 1997;26:318–26.
Stav G, Blaustein L, Margalith J. Experimental evidence for predation risk sensitive oviposition by a mosquito. Culiseta longiareolata Ecol Entomol. 1999;24:202–7.
Ikeshoji T, Mulla MS. Overcrowding factors of mosquito larvae: Isolation and chemical identification. Environ Entomol. 1974;3:482–6.
Allan SA, Kline DL. Larval rearing water and preexisting eggs influence oviposition by Aedes aegypti and Ae. albopictus (Diptera:Culicidae). J Med Entomol. 1998;35:943–7.
Xia S, Dweck HK, Lutomiah J, Sang R, McBride CS, Rose NH, et al. Larval sites of the mosquito Aedes aegypti formosus in forest and domestic habitats in Africa and the potential association with oviposition evolution. Ecol Evol. 2021;11:16327–43.
Do Nascimento JF, Palioto-Pescim GF, Pescim RR, Suganuma MS, Zequi JA, Golias HC. Influence of abiotic factors on the oviposition of Aedes (Stegomyia) aegypti (Diptera: Culicidae) in Northern Paraná. Brazil Int J Trop Insect Sci. 2022;42:2215–20.
Bédhomme S, Agnew P, Sidobre C, Michalakis Y. Pollution by conspecifics as a component of intraspecific competition among Aedes aegypti larvae. Ecol Entomol. 2005;30:1–7.
Von Dungern P, Briegel H. Protein catabolism in mosquitoes: ureotely and uricotely in larval and imaginal Aedes aegypti. J Insect Physiol. 2001;47:131–41.
Gao H, Cui C, Wang L, Jacobs-Lorena M, Wang S. Mosquito microbiota and implications for disease control. Trends Parasitol. 2020;36:98–111.
Getis A, Morrison AC, Gray K, Scott TW. Characteristics of the spatial pattern of the dengue vector, Aedes aegypti, in Iquitos, Peru. In: Rey S, Anselin L, editors. Perspectives on spatial data analysis. Advances in spatial science. Berlin: Springer; 2010. p. 203–25.
Chandel K, Mendki MJ, Parikh RY, Kulkarni G, Tikar SN, Sukumaran D, et al. Midgut microbial community of Culex quinquefasciatus mosquito populations from India. PLoS ONE. 2013;8:e80453.
Gusmão DS, Santos AV, Marini DC, Bacci M Jr, Berbert-Molina MA, Lemos FJ. Culture-dependent and culture-independent characterization of microorganisms associated with Aedes aegypti (Diptera: Culicidae) (L.) and dynamics of bacterial colonization in the midgut. Acta Trop. 2010;115:275–81.
Mosquera KD, Martinez Villegas LE, Pidot SJ, Sharif C, Klimpel S, Stinear TP, et al. Multiomic analysis of symbiotic bacteria associated with Aedes aegypti breeding sites. Front Microbiol. 2021;12:703711.
Yadav KK, Bora A, Datta S, Chandel K, Gogoi HK, Prasad GB, et al. Molecular characterization of midgut microbiota of Aedes albopictus and Aedes aegypti from Arunachal Pradesh. India Parasit Vectors. 2015;8:641.
Fader JE, Juliano SA. Oviposition habitat selection by container-dwelling mosquitoes: responses to cues of larval and detritus abundances in the field. Ecol Entomol. 2014;39:245–52.
Merritt RW, Dadd RH, Walker ED. Feeding behavior, natural food, and nutritional relationships of larval mosquitoes. Annu Rev Entomol. 1992;37:349–74.
Murrell EG, Damal K, Lounibos LP, Juliano SA. Distributions of competing container mosquitoes depend on detritus types, nutrient ratios, and food availability. Ann Entomol Soc Am. 2011;104:688–98.
Travanty NV, Apperson CS, Ponnusamy L. A diverse microbial community supports larval development and survivorship of the Asian tiger mosquito (Diptera: Culicidae). J Med Entomol. 2019;56:632–40.
Koenraadt CJM, Majambere S, Hemerik L, Takken W. The effects of food and space on the occurrence of cannibalism and predation among larvae of Anopheles gambiae sl. Entomol Exp Appl. 2004;112:125–34.
Fonseca DM, Kaplan LR, Heiry RA, Strickman D. Density-dependent oviposition by female Aedes albopictus (Diptera: Culicidae) spreads eggs among containers during the summer but accumulates them in the fall. J Med Entomol. 2015;52:705–12.
Lyimo EO, Takken W, Koella JC. Effect of rearing temperature and larval density on larval survival, age at pupation and adult size of Anopheles gambiae. Entomol Exp Appl. 1992;63:265–71.
Livdahl TP, Koenekoop RK, Futterweit SG. The complex hatching response of Aedes eggs to larval density. Ecol Entomol. 1984;9:437–42.
Bara J, Rapti Z, Cáceres CE, Muturi EJ. Effect of larval competition on extrinsic incubation period and vectorial capacity of Aedes albopictus for dengue virus. PLoS ONE. 2015;10:e0126703.
Alto BW, Lounibos LP, Mores CN, Reiskind MH. Larval competition alters susceptibility of adult Aedes mosquitoes to dengue infection. Proc Royal Soc B. 2007;275:463–71.
Alto BW, Lounibos LP, Higgs S, Juliano SA. Larval competition differentially affects arbovirus infection in Aedes mosquitoes. Ecology. 2005;86:3279–88.
Ong SQ, Jaal Z. Investigation of mosquito oviposition pheromone as lethal lure for the control of Aedes aegypti (L.) (Diptera: Culicidae). Parasit Vectors. 2015;8:28.
Starratt AN, Osgood CE. An oviposition pheromone of the mosquito Culex tarsalis: diglyceride composition of the active fraction. Biochim Biophys Acta Lipids Lipid Metab. 1972;280:187–93.
Wang F, Delannay C, Daniella G, Ligang D, Shuai G, Xiao L, et al. Cartography of odor chemicals in the dengue vector mosquito (Aedes aegypti L., Diptera/Culicidae). Sci Rep. 2019;9:8510.
Nyasembe VO, Torto B. Volatile phytochemicals as mosquito semiochemicals. Phytochem lett. 2014;8:196–201.
Nyasembe VO, Tchouassi DP, Pirk CW, Sole CL, Torto B. Host plant forensics and olfactory-based detection in Afro-tropical mosquito disease vectors. PLoS Negl Trop Dis. 2018;12:e0006185.
Wooding M, Naudé Y, Rohwer E, Bouwer M. Controlling mosquitoes with semiochemicals: a review. Parasit Vectors. 2020;13:80.
Dormont L, Bessière JM, Cohuet A. Human skin volatiles: a review. J Chem Ecol. 2013;39:569–78.
Mwingira V, Mboera LE, Dicke M, Takken W. Exploiting the chemical ecology of mosquito oviposition behavior in mosquito surveillance and control: a review. J Vector Ecol. 2020;45:155–79.
Ignell R, Hill SR. Malaria mosquito chemical ecology. Curr Opin Insect Sci. 2020;40:6–10.
Wondwosen B, Hill SR, Birgersson G, Seyoum E, Tekie H, Ignell R. A(maize)ing attraction: gravid Anopheles arabiensis are attracted and oviposit in response to maize pollen odours. Malar J. 2017;16:39.
Wondwosen B, Birgersson G, Tekie H, Torto B, Ignell R, Hill SR. Sweet attraction: sugarcane pollen-associated volatiles attract gravid Anopheles arabiensis. Malar J. 2018;17:90.
Du YJ, Millar JG. Electroantennogram and oviposition bioassay responses of Culex quinquefasciatus and Culex tarsalis (Diptera: Culicidae) to chemicals in odors from Bermuda grass infusions. J Med Entomol. 1999;36:158–66.
Bokore GE, Svenberg L, Tamre R, Onyango P, Bukhari T, Emmer A, et al. Grass-like plants release general volatile cues attractive for gravid Anopheles gambiae sensu stricto mosquitoes. Parasit Vectors. 2021;14:552.
Wondwosen B, Birgersson G, Seyoum E, Tekie H, Torto B, Fillinger U. Rice volatiles lure gravid malaria mosquitoes, Anopheles arabiensis. Sci Rep. 2016;6:37930.
Asmare Y, Hill SR, Hopkins RJ, Tekie H, Ignell R. The role of grass volatiles on oviposition site selection by Anopheles arabiensis and Anopheles coluzzii. Malar J. 2017;16:65.
Torres-Estrada JL, Meza-Alvarez RA, Cibrián-Tovar J, Rodríguez-Lopez MH, Arredondo-Jiménez JI, Cruz-López L, et al. Vegetation-derived cues for the selection of oviposition substrates by Anopheles albimanus under laboratory conditions. J Am Mosq Control Assoc. 2005;21:344–9.
Millar JG, Chaney JD, Mulla MS. Identification of oviposition attractants for Culex quinquefasciatus from fermented Bermuda grass infusions. J Am Mosq Control Assoc. 1992;8:11–7.
Cooperband MF, McElfresh JS, Millar JG, Carde RT. Attraction of female Culex quinquefasciatus Say (Diptera: Culicidae) to odors from chicken feces. J Insect Physiol. 2008;54:1184–92.
Hwang YS, Schultz GW, Axelrod H, Kramer WL, Mulla MS. Ovipositional repellency of fatty acids and their derivatives against Culex and Aedes mosquitoes. Environ Entomol. 1982;11:223–6.
Wondwosen B, Dawit M, Debebe Y, Tekie H, Hill SR, Ignell R. Development of a chimeric odour blend for attracting gravid malaria vectors. Malar J. 2021;20:262.
Buckner EA, Williams KF, Ramirez S, Darrisaw C, Carrillo JM, Latham MD, et al. A field efficacy evaluation of In2Care mosquito traps in comparison with routine integrated vector management at reducing Aedes aegypti. J Am Mosq Control Assoc. 2021;37:242–9.
We would like to thank Betelehem Wondwosen for her technical support during the GC-EAD analysis.
Open access funding provided by Swedish University of Agricultural Sciences. This project work was funded by the Department of Plant Protection Biology, Swedish University of Agricultural Sciences, SLU. The funder has had no role in the design of the study and collection, analysis, and interpretation of data, or in writing the manuscript.
Ethics approval and consent to participate
Consent for publication
The authors declare that they have no competing interests.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Multi-choice assay used to assess oviposition preference of Aedes aegypti to conspecific-conditioned aquatic stage water. a. The placement of the artificial oviposition sites (triple cups) within a BugDorm-1 cage. b. The construction of the triple cups, allowing olfactory cues, but no other sensory stimuli, to perfuse the assay. Figure S2. Oviposition site selection by gravid Aedes aegypti in response to pupae-conditioned water. The lowercase letters indicate no significant differences (P > 0.05), as determined by an ANOVA followed by a Tukey post-hoc test. Errors bars represent the standard error of the mean. Figure S3. Dual-choice oviposition assay used to evaluate choice and egg-laying of Aedes aegypti to synthetic blends. Figure S4. Oviposition choice of gravid Aedes aegypti to solvent controls (hexane) in a dual-choice assay. Gravid Ae. aegypti demonstrated no behavioural preference for either side of the oviposition assay (ANOVA followed by a Tukey post-hoc test). Error bars represent the standard error of the mean.
About this article
Cite this article
Khan, Z., Bohman, B., Ignell, R. et al. Odour-mediated oviposition site selection in Aedes aegypti depends on aquatic stage and density. Parasites Vectors 16, 264 (2023). https://doi.org/10.1186/s13071-023-05867-1