Time-of-day of blood-feeding: effects on mosquito life history and malaria transmission

Aidan J O’Donnell; Samuel S C Rund; Sarah E Reece

doi:10.1186/s13071-019-3513-9

. 2019 Jul 2;12:301. doi: 10.1186/s13071-019-3513-9

Time-of-day of blood-feeding: effects on mosquito life history and malaria transmission

Aidan J O’Donnell ^1,^✉, Samuel S C Rund ², Sarah E Reece ¹

PMCID: PMC6604169 PMID: 31262362

Abstract

Background

Biological rhythms allow organisms to compartmentalise and coordinate behaviours, physiologies, and cellular processes with the predictable daily rhythms of their environment. There is increasing recognition that the biological rhythms of mosquitoes that vector parasites are important for global health. For example, whether perturbations in blood foraging rhythms as a consequence of vector control measures can undermine disease control. To address this, we explore the impacts of altered timing of blood-feeding on mosquito life history traits and malaria transmission.

Methods

We present three experiments in which Anopheles stephensi mosquitoes were fed in the morning or evening on blood that had different qualities, including: (i) chemical-induced or (ii) Plasmodium chabaudi infection-induced anaemia; (iii) Plasmodium berghei infection but no anaemia; or (iv) stemming from hosts at different times of day. We then compared whether time-of-day variation in blood meal characteristics influences mosquito fitness proxies relating to survival and reproduction, and malaria transmission proxies.

Results

Mosquito lifespan is not influenced by the time-of-day they received a blood meal, but several reproductive metrics are affected, depending on other blood characteristics. Overall, our data suggest that receiving a blood meal in the morning makes mosquitoes more likely to lay eggs, lay slightly sooner and have a larger clutch size. In keeping with previous work, P. berghei infection reduces mosquito lifespan and the likelihood of laying eggs, but time-of-day of blood-feeding does not impact upon these metrics nor on transmission of this parasite.

Conclusion

The time-of-day of blood-feeding does not appear to have major consequences for mosquito fitness or transmission of asynchronous malaria species. If our results from a laboratory colony of mosquitoes living in benign conditions hold for wild mosquitoes, it suggests that mosquitoes have sufficient flexibility in their physiology to cope with changes in biting time induced by evading insecticide-treated bed nets. Future work should consider the impact of multiple feeding cycles and the abiotic stresses imposed by the need to forage for blood during times of day when hosts are not protected by bed nets.

Keywords: Biological rhythm, Circadian rhythm, Fitness, Reproduction, Survival, Fecundity, Plasmodium berghei, Plasmodium chabaudi, Anopheles stephensi

Background

Daily rhythms are a ubiquitous feature of life [1]. For example, circadian clocks are thought to enable organisms to coordinate with environmental periodicity in factors such as light/dark, humidity, UV exposure [2]. Interactions with predators, prey and hosts (in the case of parasites) also follow daily rhythms [3–5]. How daily rhythms, whether they are clock-controlled or direct responses to rhythmic environmental cues, shape, and are shaped by interactions between organisms is poorly understood. We address this by examining the consequences of daily rhythms in the interactions between vectors, their hosts, and their parasites. Specifically, we ask how the time-of-day that mosquitoes blood feed combines with the timing (phase) of rhythms in hosts and with malaria infection to shape vector fitness and disease transmission. Given reports that some mosquito populations have altered the time-of-day they bite (likely in response to the use of insecticide-treated bed nets) [6–13], exploring the consequences of perturbed blood foraging rhythms for mosquito fitness and malaria transmission is urgently required.

Mosquitoes exhibit periodicity in many fitness determining activities, including sugar feeding, the formation of mating swarms, insecticide resistance and blood-feeding [14, 15]. In keeping with this, ~ 20% of the Anopheles gambiae genome is expressed in patterns following daily rhythms [16]. Thus, the circadian clock enables mosquitoes to coordinate the timing of the physiological, cellular and molecular processes that underpin behaviours, with rhythms in the abiotic environment and/or other internal processes [2, 17]. For example, Anopheline mosquitoes are primarily night-biters [15, 18, 19] and processes associated with being active and foraging at night, including glycolysis, energy sensing and nutrient mobilization are upregulated in concert [16, 20]. Many genes, however, are not clock-regulated but still follow daily rhythms (including some An. gambiae odorant-binding proteins) and are driven by a direct response to light or dark [21]. Indeed in both An. gambiae and Aedes aegypti, more rhythmic genes are detected under light:dark conditions than dark:dark conditions [21, 22].

A key benefit of clock-control is that organisms can anticipate dawn/dusk and prepare in advance by up- or downregulating physiological processes. For example, processes required to cope with a blood meal are upregulated in the mosquito’s active phase (night time for Anopheles sp.) [14, 16]. This includes catalase and other factors used to detoxify reactive oxygen species (ROS) generated as a product of blood (heme) digestion, and members of the V-ATPase complex which drive water excretion to minimise the 3-fold increase in volume that a blood meal brings [23, 24]. Exposure to ROS increases mortality and reduces clutch size of mosquitoes [23, 25, 26]. Further, as a consequence of the detoxification of blood meal induced ROS, there is a proliferation of mosquito gut microbiota [27] which have complex interactions with parasite infection [28] that may vary in line with time-of-day a blood meal is taken. In addition to rhythms in processes associated with foraging, the activities and locations of immune effectors cycle throughout the day. For example, immune defences are upregulated during the day in diurnal insects, such as Drosophila [29, 30]. Whether immune defences peak at night in nocturnal mosquitoes is unknown but some immune genes implicated in interactions with malaria parasites are expressed with circadian rhythms [16]. How circadian rhythms in insect immune defences relate to protection from infection or the severity of disease is unclear. For instance, Drosophila challenged with Pseudomonas aeruginosa at night are more likely to survive the infection than those challenged in the day. However, perturbation of clock genes to generate arrhythmic mutant flies can result in both decreased survival or enhanced survival depending on the specific genes modified [31]. Further, there are complex consequences of challenging An. stephensi with E. coli or the malaria parasite P. chabaudi at different times of day [32, 33].

Given the potential for circadian rhythms to influence the ability of mosquitoes to cope with a blood meal and with parasites, the time-of-day that mosquitoes forage has implications for both mosquito fitness and disease transmission. These consequences are likely to be complex [14]. If feeding in the daytime means that mosquitoes are less able to cope with the osmotic and oxidative costs of blood, their fecundity and survival should suffer. Indeed, mosquitoes in poor condition as a consequence of feeding in the day may have compromised immune defence and this might explain recent observations that day-fed An. stephensi harbour higher densities of P. chabaudi than night-fed mosquitoes (although parasite rhythms also mediate this effect) [33]. Alternatively, ROS is a key player in insect immune responses and so, if day-fed mosquitoes do not manage their ROS efficiently, they may suffer collateral damage but also benefit from enhanced parasite defence. Furthermore, it is also necessary to recognise that mosquitoes feed on hosts that have their own circadian rhythms [14]. This includes rhythms in red blood cell composition and density, hematocrit, amino acid composition and immune effectors [34–39]. Thus, rhythms in the composition of mammalian blood could exacerbate (or reduce) the effects of a daytime blood meal on mosquito survival and fecundity.

Clearly, predicting the net effects of how host rhythms and vector rhythms interact to shape malaria transmission is challenging but important. Such interactions could shape the probability and intensity of infection in mosquitoes as well as mosquito population dynamics. Here, three experiments are described that probe the consequences, under a variety of scenarios, of time-of-day-specific blood-feeding for proxies estimating the fitness of mosquitoes and malaria parasites. The aims are to determine: (i) if the timing of a blood meal affects mosquito survival and fecundity; (ii) whether the effects of time-of-day are exacerbated by other characteristics of host blood or malaria infection; and (iii) the consequences of blood-feeding at different times of day for malaria transmission.

Methods

All experiments examine metrics of mosquito fecundity and lifespan in response to perturbing the time-of-day (morning) or (evening) that mosquitoes receive a blood meal, but differ in the following respects. The first experiment (“blood quality and host time”, Fig. 1a) includes the effects of both host time-of-day and feeding on blood from anaemic versus control mice. To further probe a role for blood quality, the second experiment (“blood quality”, Fig. 1b) uses a different approach to examine the effects of feeding on anaemic blood but does not consider host time-of-day. The third experiment (“infection,” Fig. 1c) focuses on Plasmodium berghei infection of mosquitoes.

Fig. 1 — Experimental designs. For all experiments, groups of mosquitoes differ by the time-of-day they received a blood meal. Each experiment probed the effects of further perturbations of host blood: including chemically induced anaemia and host time-of-day (Experiment 1, a); malaria infection induced anaemia (Experiment 2, b); and malaria infection of mosquitoes (Experiment 3, c)

Mice

For all experiments, hosts were 10–12-week-old MF1 male mice housed at 21 °C with ad libitum food and drinking water supplemented with 0.05% para-aminobenzoic acid (to supplement parasite growth). Mice were housed in groups of five in either 12:12 light:dark (LD; lights on at 07:00 GMT, lights off at 19:00 GMT) or inverted dark:light photocycle (DL; lights on at 19:00 GMT, lights off at 07:00 GMT) depending on the experiment. Mice were entrained to their respective light schedules for at least 21 days prior to mosquito blood feeds. Prior to donating a blood meal, each mouse was anaesthetized (17% Dormitor, 13% Vetelar, 70% PBS administered at 4 µl/g) and then exposed to a single cage of mosquitoes.

Mosquitoes

All Anopheles stephensi mosquitoes were maintained under standard insectary conditions of 27 ± 1 °C, 70% relative humidity and a 12:12 light:dark photocycle, with lights on at 07:00 GMT (ZT0) and lights off at 19:00 GMT (ZT12) (ZT0, Zeitgeber Time 0, is defined as time of lights on). Larvae were reared at a density of ~ 250 larvae per 1.5 l of distilled water. Between 12 and 14 days after hatching, pupae were transferred to emergence cages in incubators (27 ± 1 °C, 60 ± 5% relative humidity) with one-hour light ramping to simulate a dawn (starting at 07:00 GMT; ZT0) and dusk (19:00 GMT; ZT12). Mosquitoes were supplied with ad libitum access to 10% fructose solution supplemented with 0.05% paraminobenzoic acid. In the second experiment only, mosquitoes were treated with antibiotics (0.05% gentamicin) administered via their fructose solution 4–5 days before blood meals. For all experiments, female mosquitoes were randomly selected from 3–4 emergence cages, transferred to 2 l holding cages and starved of fructose solution for 24 h before their blood meals. Cages contained 15–85 mosquitoes (depending on the sampling regime of each experiment). Regardless of mosquito number, all mosquitoes were able to blood feed until satiated. For all feeds, each cage of females was exposed to an anaesthetized mouse for 30 min in a light setting that matched the mosquito time-of-day (i.e. morning-fed mosquitoes were fed during lights on and evening feeds were performed under dim red light). Unfed females were removed from the cages (< 5 per cage in all cases). After feeding, mosquitoes were housed in incubators at temperatures of either 20.5 or 26.0 °C (± 0.5 °C), depending on the experiment.

Experimental designs

Experiment 1: blood quality and host time

Mosquito cages were randomly assigned to receive a blood meal in their morning 09:00 GMT (ZT2) or evening 21:00 GMT (ZT14). These feed times are analogous to the mosquito resting period (morning) or active period (evening) as evident from wild caught and laboratory-based studies (Fig. 2, [40–42]). Within each feeding time, cages were allocated to a further four groups, based on host treatment (anaemic or control mice) and host time-of-day [morning mice (ZT2) or evening mice (ZT14)]. The availability of mice experiencing their morning or evening to feed to mosquitoes in their morning or evening was achieved by housing mice in room with LD and DL lighting schedules. This resulted in an experiment with a 2 × 2 × 2 design: eight groups varying by feed time (morning/evening), host blood treatment (anaemic/control), and host time (morning/evening) (Fig. 1a). Note, this is the only experiment that perturbs host time-of-day.

Fig. 2 — Blood feed timing. Daily flight activity of lab reared *An. stephensi* mated females (modified from [42]) showing that mosquito flight activity peaks after dusk (ZT12) with a second smaller peak before dawn (ZT0). Wild-caught mosquitoes also show this pattern, with slight variations to the size of the dusk peak depending on monsoon season [40, 41]. Shading represents timing of morning (orange) and evening (grey) blood meals in experiments 1–3. This placed the evening feeds during the mosquito’s active period and the morning feeds during the mosquito’s rest period

Anaemia was induced in half of the mice by intraperitoneal injection of 125 mg/kg of phenylhydrazine 3 days before feeding to mosquitoes. The control mice received a sham injection of 100 µl PBS. On the day of feeding, red blood cell (RBC) counts (×10⁹ ml⁻¹) for control mice (7.48 ± 0.13 SE) were almost 2-fold higher than for phenylhydrazine treated hosts (3.80 ± 0.12 SE; t = 21.27, df = 45.67, P < 0.001). Each cage contained 50 mosquitoes and each of the 8 treatment groups contained 6 cages. On day 2 post-blood meal (PBM), mosquitoes were allocated to individual housing (50 ml falcon tubes with ad libitum access to 10% glucose solution via a 1.5 ml microcentrifuge tube feeder). Fecundity and mortality were tracked for 20 mosquitoes from each cage (960 total). Each female was given a 30 mm diameter Petri dish lined with filter paper and 3 mm depth of distilled water as an oviposition habitat. Mosquitoes were checked daily and if eggs were present, the egg dish was replaced. Egg bowls were photographed at the time of removal (for clutch size counts) incubated for 6 days and then photographed again so that all hatched larvae (alive and dead) could be counted (to estimate hatch rate). For all females (that did or did not lay) egg bowls were removed on day 9 PBM.

Additionally, the volume and density of blood meals were estimated for 10 randomly chosen mosquitoes from each cage (480 total) 2 hours after their blood meal. The right wing of each mosquito was photographed, and the abdomen removed and homogenised in 500 µl drabkins solution for ~ 30 min [43]. Samples were split into two 200 µl sub-samples and optical density (OD) read by a spectrophotometer at 540 nm (each mosquito was read in duplicate, and an average taken). To generate control series for each cage, 8 µl of blood was removed from each mouse used to feed mosquitoes at the time of feeding and used to generate 4 µl, 1 µl, 0.8 µl and 0.4 µl standards. Host RBC density readings (cells per µl) were also obtained at the time of feeding to calculate the RBC density of the blood meal. Wing length was obtained from the photographs, converted to mm and used to control for any potential differences in blood meal volume and density due to variation in body size (using the software package ImageJ [44]).

Experiment 2: blood quality

Here, instead of phenylhydrazine treatment, blood quality was perturbed by using malaria infection to generate anaemia. Mosquito cages were randomly assigned to morning 09:00 GMT (ZT2) or evening 21:00 GMT (ZT14) feed times. At each feeding time, half the cages were exposed to anaemic or (uninfected) control mice. This resulted in an experiment with a 2 × 2 design: four groups varying by the timing of their blood meal (morning/evening) and blood treatment (anaemic/control) (Fig. 1b). Note, host time-of-day was standardised by housing mice in two rooms with inverted light schedules (DL and LD), enabling both the morning- and evening-fed mosquitoes to feed on hosts experiencing their evening (host ZT14). Six cages were fed, at each time point, on control mice and nine cages, at each time point, on anaemic mice. Each cage exposed to control mice contained 15 mosquitoes and each cage exposed to anaemic mice contained 20 mosquitoes. Mortality was tracked as for Experiment 1 (but for 10 individuals per cage; 300 total) and egg dishes were provided until day 14 PBM.

All feeds occurred on mice at day 11 post-infection (PI) after infection with 1 × 10⁶ P. chabaudi CR parasitized RBCs or sham infection (controls; 100 µl PBS). Plasmodium chabaudi has a synchronous asexual cycle so donor mice were used from each room (DL and LD) to ensure that all hosts were infected with rings (i.e. parasite and host rhythms were phase matched; [45]). By day 11 PI, significant anaemia had occurred (mean RBC density × 10⁹ ml⁻¹: Control = 7.88 (± 0.16 SE), anaemic = 4.44 (± 0.10 SE); t = 18.77, df = 19.28, P < 0.001) and hosts were mounting strong immune responses, so the parasite was not able to establish an infection in mosquitoes (parasite mating is very vulnerable to suboptimal conditions in the blood meal [46]). Thus, mosquitoes received poor quality blood as a result of a more ecologically realistic perturbation than PHZ, without the confounding effects of becoming infected themselves. This was verified by examining 10 randomly selected mosquitoes from each cage exposed to anaemic mice on day 14 PBM. Specifically, the midgut of each mosquito was dissected, stained for two minutes in 0.5% mercurochrome, washed in PBS and total oocysts per midgut were counted via microscopy. No oocysts were detected.

Experiment 3: infection

Mosquito cages were randomly assigned to four groups. Two groups received their blood meal in the morning 10:00 GMT (morning, ZT3) and the others were fed in the evening at 20:00 GMT (evening, ZT13). At each feed time, half of the cages were exposed to Plasmodium berghei infected mice or naïve (uninfected) control mice. This resulted in an experiment with a 2 × 2 design: four groups varying by the timing of their blood meal (morning/evening) and blood treatment (infected/uninfected) (Fig. 1c). Note that time-of-day for parasites/hosts and mosquitoes is synonymous; morning-fed mosquitoes received blood from hosts also experiencing their morning, and vice versa for evening-fed mosquitoes. At each time point, six cages were fed on infected mice and four fed cages on uninfected mice.

All feeds occurred on mice at day 6 PI after inoculation with 1 × 10⁵ P. berghei parasitized RBCs or sham infection (controls; 100 µl PBS). Infections (and sham injections) were staggered by 10 h to ensure that morning- and evening-fed mosquitoes were exposed to infections of the same age (144 h). Plasmodium berghei was chosen because its asexual cycle is asynchronous, ensuring that morning- and evening-fed mosquitoes did not receive significantly different stage distributions of asexual parasites (feed time:parasite stage; χ²₄ = 1.28, P = 0.29; Fig. 3a) or gametocyte densities/ages (mean gametocyte density × 10⁷ ml⁻¹: morning = 3.93 (± 0.14 SE), evening = 3.80 (± 0.1 SE); t = 0.77, df = 10, P = 0.46; Fig. 3b). On day 6 PI, P. berghei had not significantly reduced the RBC density of hosts (mean RBC density × 10⁹ ml⁻¹: Control = 8.17 (± 0.08 SE), Infected = 7.85 (± 0.18 SE); t = 1.64, df = 14.71, P = 0.12).

Fig. 3 — Composition of *P. berghei* parasites in mice used to infect mosquitoes in experiment 3. Shown are the means ± SE parasite stage proportions (a) and gametocyte density (b) from infected hosts used for blood meals. Donors were sampled at the time of blood meals either in the morning (AM; 10:00 GMT; ZT3) or evening (PM; 20:00 GMT; ZT13) (n = 6)

At the time of feeding, each cage contained 85 mosquitoes. After the blood meal, 15 mosquitoes from cages fed on infected mice were removed (180 total) and used to monitor oocyst prevalence and density as for Experiment 2. To track mosquito fecundity and mortality, a subset of 15 randomly selected females were removed from each cage (300 total) 2 days PBM and housed individually in 200 ml cups with ad libitum access to 10% fructose solution. On day 3 PBM, each female was given a 30 mm diameter Petri dish lined with filter paper and 3 mm depth of distilled water as an oviposition habitat. Mosquitoes were checked daily until death, if eggs were present the egg dish was replaced (up until day 21 PBM).

Data analysis

R version 2.6.1 [47] was used for all analyses. Model simplification was carried out by stepwise deletion of the least significant term and only minimal models are reported. Measurements made from mice at the time of feeding (red blood cell counts and parasite stage composition and densities), and time-of-day differences in infection load for mosquitoes were analysed with Studentʼs t-test. Mosquito fecundity metrics, proportion of females that laid and hatch rate, were analysed using generalised linear mixed-effects models with binomial error structures. Clutch size and blood meal measures were analysed using linear mixed effect models. In both types of linear models, identity of the mosquito cage was included as a random effect. All models met model assumptions: independence of data points, normality of residuals and homogeneity of variances (confirmed through assessing the model plots, the Shapiro–Wilk test and Bartlett’s test). Cox proportional hazard models with mosquito identity nested within cage as random effects (frailty model) were used to estimate the effects of feed time and host blood manipulations on the time taken to lay and lifespan (coxme package in R [48]). All Cox models model met the proportional hazards assumptions based on Schoenfeld’s residuals (evaluated using the ‘cox.zph’ function R; P > 0.1 for all variables). Clutch size of mosquitoes that laid and its interactions with experimental treatments was also controlled for because the data indicated considerable heterogeneity in clutch size, and trade-offs between survival and reproduction have been reported [49, 50] and may depend on resource availability, which may vary as a consequence of perturbations of blood quality. For this reason, mosquitoes that did not lay eggs were excluded from time to lay, clutch size and lifespan analyses. For all analyses, main effects and two-way interactions were investigated.

Results

We carried out three experiments to determine how the timing of receiving a blood meal affects aspects of mosquito survival and fecundity, and whether qualities of host blood or malaria infection modulate the effects of the time-of-day that mosquitoes feed.

Experiment 1: blood quality and host time

This experiment (Fig. 1a) recognises that hosts have circadian rhythms in blood composition and was designed to address if host time-of-day and blood quality (chemical induced anaemia) interact with mosquito feeding time-of-day to shape the following parameters (see Table 1 for a summary).

Table 1.

Summary of statistical results for analyses in Experiment 1, Experiment 2 and Experiment 3

Fitness metric	Statistical results for each term in model
Experiment 1
Blood meal volume	Sig: Blood quality
Blood meal volume	Non-Sig: Feed time:host time; Feed time:blood quality; Host time:blood quality; Feed time; Host time
Blood meal density	Sig: Host time:blood quality
Blood meal density	Non-Sig: Feed time:host time; Feed time:blood quality; Feed time
Proportion laid	Sig: Feed time
Proportion laid	Non-Sig: Host time:blood quality; Feed time:host time; Feed time:blood quality; Host time; Blood quality
Time to lay	Sig: Feed time
Time to lay	Non-Sig: Host time; Blood quality
Clutch size	Sig: Feed time:blood quality
Clutch size	Non-sig: Feed time:host time; Host time:blood quality; Host time
Hatch rate	Sig: na
Hatch rate	Non-sig: Feed time:host time; Feed time:blood quality; Host time:blood quality; Feed time; Host time; Blood quality
Lifespan	Sig: na
Lifespan	Non-sig: Host time; Feed time; Blood quality
Experiment 2
Proportion laid	Sig: na
Proportion laid	Non-Sig: Feed time:blood quality; Blood quality; Feed time
Time to lay	Sig: na
Time to lay	Non-Sig: Feed time:blood quality; Blood quality; Feed time
Clutch size	Sig: Blood quality
Clutch size	Non-sig: Feed time:blood quality; Feed time
Lifespan	Sig: na
Lifespan	Non-sig: Feed time; Blood quality
Experiment 3
Malaria prevalence & intensity	Sig: Infected/uninfected blood
Malaria prevalence & intensity	Non-Sig: Feed time
Proportion laid	Sig: Infection status
Proportion laid	Non-Sig: Infection status:feed time; Feed time
Time to lay	Sig: Infection status
Time to lay	Non-Sig: Infection status:feed time; Feed time
Clutch size	Sig: na
Clutch size	Non-sig: Infection status:feed time; Feed time; Infection status
Lifespan	Sig: Infection status
Lifespan	Non-sig: Feed time

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Notes: Terms that significantly affected the mosquito fitness metric in question are highlighted in italics. Interactions between terms are indicated by ‘:’ and main effects are not included for terms involved in significant interactions

Blood meal: volume and density

There was no significant effect of feed time (χ²₇ = 1.02, P = 0.31), host time (χ²₅ = 0.01, P = 0.91), or their interaction (χ²₉ = 0.40, P = 0.53) on the volume of the blood meal. The effect of host blood quality was not significantly influenced by interactions with feed time (χ²₈ = 0.75, P = 0.39) or host time (χ²₆ = 2.29, P = 0.13). However, mosquitoes that fed on anaemic hosts took up a greater volume of blood than those that fed on control hosts (mean ± SE blood meal volume (µl) per mm wing length: control = 0.26 ± 0.01), anaemic = 0.33 ± 0.01; χ²₄ = 17.90, P < 0.0001; Fig. 4a). There was also a borderline significant interaction between host time and host blood quality on the RBC density of the blood meal (χ²₆ = 4.30, P = 0.038; Fig. 4b). Specifically, mosquitoes that fed on control hosts consumed more RBCs than those that fed on anaemic hosts, especially when fed on hosts that experienced their morning (mean ± SE × 10⁶; control hosts: morning = 2.11 ± 0.94, evening = 1.77 ± 0.75; anaemic hosts: morning = 1.24 ± 0.54, evening = 1.29 ± 0.60). There was no significant effect of feed time (χ²₇ = 0.66, P = 0.42), nor its interactions with host blood quality (χ²₉ = 0.65, P = 0.42) or host time (χ²₈ = 3.25, P = 0.07) on the RBC of the blood meal.

Fig. 4 — Blood meal volume (a) and blood meal RBC density (b) in response to perturbations of host blood quality and host time-of-day (Experiment 1). Mean ± SE, adjusted for body size. AM indicates morning for hosts and parasites, at 09:00 GMT (ZT 2) and PM indicates 21:00 GMT (ZT 14). Anaemia was induced in hosts by phenylhydrazine (125 mg/kg injected intraperitoneally)

Reproduction: proportion laid

Neither host blood quality (χ²₅ = 1.60, P = 0.21), host time (χ²₄ = 2.44, P = 0.12), or their interaction (χ²₈ = 0.02, P = 0.89) significantly affected the probability each mosquito laid. However, feed time did matter, with mosquitoes that fed in the morning more likely to lay than those that fed in the evening (mean ± SE proportion of females that laid: morning = 0.82 ± 0.02, evening = 0.65 ± 0.02; χ²₃ = 27.56, P < 0.0001; Fig. 5a). However, feed time did not significantly interact with either host blood quality (χ²₆ = 0.41, P = 0.52) or host time (χ²₇ = 0.05, P = 0.83).

Fig. 5 — Mosquito reproduction and survival in response to perturbations of host blood quality and host time-of-day (Experiment 1). Shown are Kaplan–Meier curves for the time taken to lay (a), mean ± SE clutch size (b), and Kaplan–Meier curves for mosquito survival (c, d). AM indicates a morning feed at 09:00 GMT (ZT 2) and PM an evening feed at 21:00 GMT (ZT 14). Mosquitoes that did not lay are omitted from b, c and d. Due to the negative effect of clutch size on survival Kaplan–Meier curves for survival (c and d) were estimated based on median clutch size of 65. Lines represent time to lay event (a) and survival estimates with 95% confidence intervals in shading (c, d). Anaemia was induced in hosts by phenylhydrazine (125 mg/kg injected intraperitoneally)

Reproduction: time to lay

For mosquitoes that laid, neither host blood quality (z = 0.73, P = 0.47) or host time (z = 0.95, P = 0.34) influenced the time it took mosquitoes to lay eggs. Feed time did have an effect with mosquitoes that fed in the morning laying sooner than those that fed in the evening (mean ± SE days taken to lay since egg bowls were provided: morning = 1.15 ± 0.03, evening = 1.44 ± 0.04; evening:morning HR = 0.64 ± 0.08, z = − 5.35, P < 0.001; Fig. 5a).

Reproduction: clutch size

Clutch size was shaped by a borderline interaction between feed time and host blood quality (χ²₆ = 4.13, P = 0.042; Fig. 5b). Mosquitoes fed on control mice had higher clutch sizes than those that fed on anaemic hosts, and this difference was greatest when mosquitoes fed in the morning (mean ± SE clutch size: morning-fed: control hosts = 65.57 ± 1.77, anaemic hosts = 51.06 ± 1.70; evening-fed: control hosts = 61.88 ± 1.97, anaemic hosts = 55 ± 2.09). There was also a non-significant tendency for mosquitoes that fed on hosts experiencing their morning to have higher clutch size (mean ± SE clutch size: morning hosts = 56.36 ± 1.37, evening hosts = 59.99 ± 1.34; χ²₇ = 3.70, P = 0.054). However, this trend for an effect of host time was not modulated by feed time (χ²₈ = 3.06, P = 0.08) or host blood quality (χ²₉ = 0.03, P = 0.87).

Reproduction: hatch rate

Neither host blood quality (χ²₄ = 0.12, P = 0.73) or host time (χ²₆ = 0.02, P = 0.89) or their interaction (χ²₈ = 0.10, P = 0.75) influenced egg hatch rate. Likewise, there was no significant influence of feed time (χ²₃ = 1.31, P = 0.25) and its interactions with host blood quality (χ²₅ = 2.12, P = 0.15) and host time (χ²₇ = 0.40, P = 0.53). Mean hatch rate for all clutches was 0.69 (± 0.01 SE).

Lifespan

For mosquitoes that laid, neither host blood quality (z = 0.28, P = 0.78), host time (z = 0.75, P = 0.45) or feed time (z = − 0.10, P = 0.92) significantly influenced mortality rate (Fig. 5c–d). Clutch size was negatively associated with survival hazard (clutch HR = 0.996, z = − 2.54, P = 0.011), with smaller clutches (< 60 eggs) associated with a greater hazard than larger clutches (> 60 eggs). The median lifespan for all mosquitoes (that laid) was 13 days post-blood meal.