- Open Access
Increasing role of Anopheles funestus and Anopheles arabiensis in malaria transmission in the Kilombero Valley, Tanzania
© Lwetoijera et al.; licensee BioMed Central Ltd. 2014
- Received: 4 July 2014
- Accepted: 22 August 2014
- Published: 24 August 2014
In order to sustain the gains achieved by current malaria control strategies, robust surveillance systems that monitor dynamics of vectors and their roles in malaria transmission over time are essential. This longitudinal study demonstrates the trends in malaria vector dynamics and their relative contribution to malaria transmission in hyperendemic transmission settings in Tanzania.
The study was conducted in two villages within the Kilombero Valley, in rural Tanzania for five consecutive years (2008–2012). Seventy-two houses were selected per village and each house was sampled for mosquitoes monthly using a CDC light trap. Collected mosquitoes were assessed for species identity and sporozoite infection status using PCR and ELISA, respectively. Anopheles funestus and Anopheles arabiensis susceptibility to insecticides was assessed using WHO guidelines.
A total of 100,810 malaria vectors were collected, of which 76% were Anopheles gambiae s. l. and 24% were An. funestus. Of all An. funestus samples that amplified with PCR (n = 2,737), 97% were An. funestus s.s., 2% were Anopheles rivorulum and 1% Anopheles leesoni. Whereas for An. gambiae s.l. (n = 8,117), 93% were An. arabiensis and 7% were Anopheles gambiae s.s. The proportion of An. gambiae s.s. identified by PCR (2,924) declined from 0.2% in the year 2008 to undetectable levels in 2012. Malaria transmission intensity significantly decreased from an EIR of 78.14 infectious bites/person/year in 2008 to 35 ib/p/yr in 2011 but rebounded to 226 ib/p/yr in 2012 coinciding with an increased role of An. funestus in malaria transmission. Insecticide susceptibility tests indicated high levels of resistance in An. funestus against deltamethrin (87%), permethrin (65%), lambda cyhalothrin (74%), bendiocarb (65%), and DDT (66%). Similarly, An. arabiensis showed insecticide resistance to deltamethrin (64%), permethrin (77%) and lambda cyhalothrin (42%) in 2014.
The results indicate the continuing role of An. arabiensis and the increasing importance of An. funestus in malaria transmission, and pyrethroid resistance development in both species. Complementary vector control and surveillance tools are needed that target the ecology, behaviour and insecticide resistance management of these vector species, in order to preserve the efficacy of LLINs.
Malaria transmission in humans is sustained through vector-human interactions  and vector control interventions, such as long-lasting, insecticidal nets (LLINs), aim to break this interaction. Major promotion of LLINs in recent years has resulted in average household ownership rates and usage of LLINs of approximately 42 and 36%, respectively, in sub-Saharan Africa . In mainland Tanzania, a recent report by the Tanzania HIV and Malaria Indicator Survey (THMIS) indicates that above average LLIN ownership and usage (approximately 90 and 66%, respectively) was associated with improved malaria control and overall reduction in malaria prevalence .
One outcome of LLIN use is that, by limiting availability of human hosts [4–6], vector species composition in any given area can change considerably after a long period of LLIN use. Anopheles gambiae sensu stricto, Anopheles arabiensis and Anopheles funestus are the primary malaria vectors in sub-Saharan Africa [7, 8], often occurring sympatrically . Anopheles gambiae s.s. is often regarded as the most important vector species across Africa [9–11] and, because of its almost entirely anthropophagic and endophilic behaviour, it is the species that has been targeted most effectively by LLINs.
However, in some locations, populations of An. gambiae s.s. have developed insecticide resistance and it continues to be the dominant vector [12, 13]. In other locations, An. gambiae s.s. populations have crashed and the relative importance of the remaining vector species has shifted, with An. arabiensis becoming the major malaria vector [4, 5, 11].
Since single populations of An. arabiensis can exhibit a range of behaviours, biting and resting indoors as well as outdoors and feeding on both humans and animals, interventions that optimally target indoor resting and biting vectors often impact far less on this species [11, 14–17]. The primary vector of the An. funestus complex, An. funestus is also a very anthropophilic and endophilic mosquito and it too can be a highly efficient malaria vector [10, 18, 19].
Kilombero Valley in southern Tanzania has been subject to a large number of studies on malaria epidemiology, dating back many years, with malaria parasite prevalence rates of up to 70% and an entomological inoculation rate (EIR) of 300 infectious bites per person per year (ib/p/yr) being recorded in the 1990s, the period before the introduction of bed nets . Following the scaling up of untreated nets in the early 2000s  and insecticide-treated bed nets (ITNs) and LLINs from 2004 to 2011 [22–24], a continuous decline in malaria vector numbers and malaria transmission has been seen [3, 12]. Although the populations of An. gambiae s.s. are significantly dwindling in southern and other parts of Tanzania , the remaining populations of An. arabiensis and An. funestus appears to have shifted their blood-feeding periodicity to optimize their chances to obtain blood meal from their preferred hosts even in the time of low LLIN coverage . It is however suggested that prolonged, widespread use of LLINs is likely to favour outdoor and early biting, either as an expression of the mosquito’s innate phenotypic plasticity or possibly as a heritable, selectable trait that might be expected to increase in frequency .
The malaria vector populations in this area are subject to ongoing rigorous monitoring and herein five years of data to the end of 2012 are reported; describing changes in vector species composition and relative abundance, insecticide susceptibility and their contribution to malaria transmission following the years of widespread LLIN use since first introduced in 2004.
This study was conducted over five years between January 2008 and December 2012. A total of 72 houses from each village were randomly selected from the Ifakara Health Institute (IHI) Demographic Surveillance System household list . All selected houses were geolocated using a handheld GPS (eTrex, Vista, Garmin, USA). Mosquitoes were sampled in every house each month during 2008, 2011 and 2012 and for six months from January to June in 2009 and July to December in 2010.
Mosquito sampling and processing
Mosquitoes were sampled using miniature Center for Disease Control (CDC) light traps (model 512, USA). One CDC light trap was used overnight per house, placed 1–1.5 m from the fan above the ground close to the foot end of an occupied bed, and left to run for 12 hours (19.00-07.00) [27, 28]. For every participating house, one LLIN (Olyset, A to Z Textiles Mills, Arusha, Tanzania) was provided to protect the bed occupant where the CDC trap was set. The following morning, CDC light traps were collected and mosquitoes killed using chloroform, and identified in the field using a morphological key . Female mosquitoes were classified as being unfed, partially fed, fully fed or gravid. Subsamples of five mosquitoes from each trap for An. arabiensis and An. funestus species were individually stored inside a tube containing cotton wool and silica gel beneath for further individual molecular species identification using polymerase chain reaction (PCR) assay for the An. gambiae complex  and An. funestus group  and sporozoite infection status using enzyme-linked immunosorbent assay (ELISA)  in the laboratory (species identification for the An. funestus group did not begin until 2009).
All the sorting information and laboratory analysis results were recorded using designated data collection forms for entomological studies (Kiware et al., unpublished). In addition, variations in malaria transmission by different vector species over time were assessed and compared using the annual EIR calculated by biting rate (total collections/trap nights/year) and the proportion of females infected with sporozoites . Monthly average rainfall data for 2008–2011 were obtained from the Kilombero Valley Teak Company (approximately 15 km from Idete village), and data for year 2012 data were obtained using rain gauges installed in Namwawala village.
Insecticide susceptibility tests
Following significant increase in An. funestus population in 2012, despite extensive usage of LLIN in the study area, it was unclear whether this was due to its reduced susceptibility to the insecticides used in LLINs. The tests were conducted using WHO standard procedures and test kits for adult female mosquitoes of An. arabiensis and An. funestus in Namwawala villages from January to June 2013. As the confirmatory process, the biossays were repeated in June 2014 for both species.
Five classes of insecticides currently recommended for vector control were tested using discriminating concentrations impregnated in pre-prepared test papers as follows: deltamethrin (0.05%), permethrin (0.75%), lambda cyhalothrin (0.05%), bendiocarb (0.1%), and DDT (4%). Unfed female wild An. funestus collected using CDC light traps were used for insecticide exposure bioassays, as recommended by WHO for this difficult-to-colonize species . However, this method is limited by greater variation in susceptibility due to unknown age differences between test mosquitoes, it is simple to carry in the field with minimal infrastructure and test mosquitoes highly representative of the natural population .
Prior to exposure, morphologically identified mosquitoes were maintained on 10% glucose solution for at least five hours prior to testing; whereas, for An. arabiensis, F1 female mosquitoes two to three days old (recommended age group) were used for bioassays from reared Anopheles larvae collected from the breeding habitats in the study sites [34, 35]. Species identification was carried out after bioassays on dead mosquitoes using PCR.
A total of 100 mosquitoes were exposed per discriminating concentration in five replicates of 20 mosquitoes each, and compared to a control with same number of mosquitoes per replicate. In an exposure tube, mosquitoes were held for a total of one hour in intervals of 10, 15, 20, 30, 40, 50, and 60 minutes. After the first hour of exposure, mosquitoes were transferred to non-insecticide treated, clean, holding tubes and observed for a further 20 minutes . After 80 minutes (initial 60 min + further 20 min) of knockdown monitoring, all mosquitoes were transferred to non-insecticide treated, clean, holding tubes and kept for 24 hours and provided with 10% glucose solution, after which mortality was monitored and recorded. All these procedures were performed in the field under average ambient temperatures of 26 ± 2°C and a relative humidity of 78 ± 3% in both bioassay rounds. Percentage knockdown in the observed mosquitoes was recorded immediately for each time interval, and mosquito mortality in each bioassay was expressed as the proportion of dead mosquitoes to total exposed, for each tested insecticide. Execution and interpretation followed recently updated WHO test procedures for insecticide resistance monitoring in malaria vector mosquitoes .
Only data pertaining to An. gambiae s.l. and An. funestus were analysed, using SPSS version 20 (SPSS Inc, Chicago, USA). Data were fitted with generalized linear models (GLMs) using a negative binomial distribution with log-link function, and relative rates (RR) with 95% confidence intervals calculated to estimate yearly mean mosquito catches, relative to the reference year. Species (An. gambiae s.l. and An. funestus) were treated as predictors and total number of mosquitoes as a dependent variable; the statistical differences in dependent variables was evaluated as a function of villages (Idete and Namwawala), seasons (wet and dry) and years (2008–2012).
Insecticide susceptibility test biossay data were considered for each diagnostic concentration and year of testing. Mortality was calculated as the percentage of mosquitoes dead post 24 hours’ exposure to insecticide, and the results were assessed according to WHO testing procedure for insecticide resistance monitoring in malaria vectors . Mortality rates between 98 and 100% indicate full susceptibility, 90-97% is suggestive of resistance and requires further investigation, and mortality rates less than 90% confirm the existence of resistance.
The study approval was granted by the Ifakara Health Institutional Review Board (IHRDC/IRB/No.A-32) and the National Institute of Medical Research (NIMR/HQ/R.8a/Vol. IX/764). On first visiting each house, the benefits and possible risks associated with the study were explained to the house occupants and informed consent to proceed was requested. After consenting, the head of the house was asked to sign two copies of the informed consent forms, (retained by the head of the house and the study investigator).
Relative abundance of malaria vector species
During the five consecutive years of sampling with CDC light traps in sentinel houses, a total of 100,810 malaria vectors were collected of which 76% were Anopheles gambiae sensu lato and 24% were An. funestus. In each of the first four years (2008–2011), the proportion of An. gambiae s.l. was significantly higher than An. funestus in both study villages (p <0.0001): proportions in total catches in Namwawala were 94% (40,028) and 6% (2,398), and in Idete were 87% (24,869) and 13% (3,730) for An. gambiae s.l. and An. funestus, respectively. However, in 2012, the proportion of total catch of An. funestus was significantly higher than An. gambiae s.l. in both villages: 42% (6,622) and 58% (8,953) in Namwawala and 35% (4,479) and 65% (8,447) in Idete for An. gambiae s.l. and An. funestus, respectively, (RR (95% CI) = 1.35 (1.23-1.49), p <0.0001).
Malaria vector composition, sporozoite prevalence (S), biting rate (B) and entomological inoculation (EIR) for Anopheles gambiae s.s., Anopheles arabiensis and Anopheles funestus and their overall estimated yearly contribution to malaria transmission from year 2008–2012 in the study area
An. gambiae complex sibling species proportion
An. gambiae s.s.
No. of PCR amplifications
An. funestus group sibling species proportion
An. funestus s.s.
No. of PCR amplifications
Sporozoite prevalence (S;%)
An. gambiae s.s.
Biting rate (B; b/p/n)
An. gambiae s.s.
Entomological Inoculation Rate (EIR; ib/p/y)
An. gambiae s.s.
Of the 2,737 An. funestus samples that were identified by PCR, 97% were An. funestus s.s. (n = 2,655), 2% were Anopheles rivorulum (n = 55) and 1% Anopheles leesoni (n = 27). The species composition of An. funestus in Idete was 98% (n = 1,554) An. funestus s.s, 1.5% (n = 23) An. rivorulum and 0.4% (n = 6) An. leesoni. In Namwawala it was 98% (n = 1,133) An. funestus s.s., 0.6% (n = 7) An. rivorulum and 1.2% (n = 14) An. leesoni, (Table 1).
Seasonal variation in vector abundance
The mean number of An. funestus per trap per night in the wet and dry season of the first four years of study (2008–2011) was consistently similar in both villages. In the wet season, the mean catches (+SD) were 1.23 + 4.7 in 2008, 2.15 + 7.5 in 2009/10, 0.64 + 1.9 in 2011 compared to 1.15 + 5.2, 0.77 + 4.3 and 1.62 + 5.52 of the respective years in the dry season. In 2012, the mean catch of An. funestus, both in wet and dry seasons, was approximately six times significantly higher than in the previous years (p <0.0001): 11.75 + 45.8 and 8.3 + 25.6 of wet and dry season, respectively.
A total of 10,138 individual mosquitoes (530 An. gambiae s.s., 7,130 An. arabiensis and 2,478 An. funestus s.s.) were screened for Plasmodium falciparum sporozoites of which 75 were positive (0.74% sporozoite prevalence). Although An. gambiae s.s. was the major malaria vector with a sporozoite prevalence of 1.18% in 2008, its dominance decreased with time to zero in 2011 and 2012, following its control to undetectable levels. Conversely, the importance of An. arabiensis and An. funestus s.s was increasing with time from a sporozoite prevalence of 0.16% in 2008 to 1.47% in 2012 for An. arabiensis, and from 1.71% in 2008 to 2.2% in 2012 for An. funestus s.s.
Similarly, the EIR of An. gambiae s.s. decreased drastically from 30.70 ib/p/yr in 2008 to 0 ib/p/yr in 2012, whereas those of An. arabiensis increased approximately four times from 30.58 in 2008 to 110.9 in 2012 and that of An. funestus s.s. increased 11 times from 10.86 in 2008 to 115.10 in 2012.
Overall, the level of malaria transmission in the study villages markedly decreased with time from an EIR of 78.14 ib/p/yr in 2008 to 31.05 ib/p/yr in 2011 but overwhelmingly increased to 226 ib/p/yr in 2012, approximately seven times more than in the previous year (Table 1).
Anopheles arabiensis and Anopheles funestus insecticide susceptibility tests
In year 2013, An. arabiensis was fully susceptible to bendiocarb (100% mortality) and deltamethrin (98.3%), reduced susceptibility against DDT (97%), and confirmed resistance to permethrin (83.3%) and lambda cyhalothrin (78%), with a control mortality of 0% across all test concentrations. Similar levels of resistance were maintained across tested diagnostic concentrations in year 2014, whereby the mosquitoes were fully susceptible to bendiocarb (98% mortality) and resistant to deltamethrin (64%), permethrin (77%), and lambda cyhalothrin (42%), with a control mortality of 0% across all test concentrations.
This study provides substantial information on malaria vector dynamics and their contribution to malaria transmission in rural southern Tanzania over a five year period. Consistent with other studies, which have documented a shift in malaria vector composition and a change in malaria transmission dynamics seemingly as a result of extensive use of LLINs [4, 5, 36], this study reports a steady decrease to undetectable levels of An. gambiae s.s. with steady increase in the proportion of its sibling species An. arabiensis and a surge in the abundance of An. funestus s.s. in year 2012.
Anopheles gambiae s.s. prefers to feed and rest inside houses. This makes it more vulnerable to insecticides applied to nets (LLINs) and walls (indoor residual spraying (IRS)) while An. arabiensis, with its opportunistic feeding behaviour both on humans and animals [12, 32] and its potential to rest outside human dwellings, make it less affected by LLINs. Although, lack of outdoor mosquito collections was a major limitation of this study in explaining the shift in biting periodicity and outdoor biting, it has been recently documented elsewhere that An. arabiensis and An. funestus[25, 37] display a behavioural avoidance to contact LLINs by feeding outdoors in early part of the evening which might increase its chance to survive current interventions.
A significant increase in An. funestus abundance and EIR in 2012 is demonstrated. This shift poses great concern in malaria control efforts due to its efficiency in transmitting malaria. Historically the control of An. funestus s.s. was successful through extensive IRS, taking advantage of its highly anthropophagic and endophilic behaviour, using dieldrin in Pare, Taveta, northern Tanzania [38, 39] Malindi on the coast of Kenya, using DDT  as well as in South Africa . This is partly because they spend a longer time on insecticide-treated materials . However, the vector eventually resurged six years later due to a lack of IRS programme continuity and consolidation [40, 43]. A similar scenario was expected in this particular region, where usage of LLINs is high [3, 44].
The steady increase in An. funestus population density, despite extensive usage of LLINs in the study area, may be due to its reduced susceptibility to the insecticides used in LLINs. Recent findings from western Kenya have demonstrated similar phenomenon of resurging An. funestus populations, chiefly being due to resistance development to the pyrethroids used in LLINs .
Preliminary findings from this study demonstrated high resistance of An. funestus and An. arabiensis to pyrethroids, deltamethrin, lambda cyhalothrin and permethrin, used in Olyset LLINs, distributed in the study area in June 2011 . Overall, there was great variation of the resistance status between 2013 and 2014 in both species tested; however, the variation was surprisingly huge in An. funestus than An. arabiensis, which might be due to inconsistency in unknown age of the used wild mosquito females .
Due to the absence of organochlorine insecticide DDT and carbamate insecticide bendiocarb deployment for malaria vector control in the study area, the source of resistance in mosquitoes to these insecticides remains unknown. Although not tested in this particular study, pyrethroid (DDT and pyrethroid) carbamate cross-resistance was considered to be a probable cause of An. funestus resistance to DDT and bendiocarb, respectively, which has been proved to exist in malaria vectors elsewhere [46, 47]. In addition, the continuous and illegitimate use of DDT as a pesticide in agriculture in the region might have contaminated malaria vector breeding habitats and caused physiological resistance in mosquitoes .
Pyrethroid resistance in both species has been documented in multiple countries and regions of East Africa [45, 49, 50], southern Africa [51–54] and West Africa [55–57]. Further detailed studies are urgently required to establish current vector control operational impacts associated with this level of resistance. These findings suggest an increased contribution of these vectors to malaria transmission and hence great threat to the future use of LLINs in controlling these vectors.
The other probable cause for the observed increase in An. funestus population in this study area, which requires further investigation, might be a shift of An. funestus to outdoor and early evening and daytime biting behaviours, which increase their chances to survive and reproduce by feeding on unprotected humans, as recently documented An. funestus behaviours in Benin  and Senegal , West Africa.
In this study, both An. funestus and An. gambiae s.l. vector abundance varied with season. Increases in An. gambiae s.l. densities are facilitated by a wide range of ephemeral, sunlit, breeding habitats, such as hoof prints, rice puddles and ground depressions created during the rainy season [18, 60]. The temporary nature of these habitats tends to reduce predation rate but also allows quick development of the juvenile stages, which results in An. gambiae s.l. dominating during the rainy season . On the contrary, An. funestus prefer vegetated semi-permanent and permanent breeding habitats, such as swamps and large ponds . Anopheles funestus remained at a reasonable and detectable density across the rainy and dry seasons in the study areas and were significantly more abundant than An. gambiae s.l. in the dry season, probably due to their breeding habitat stability against desiccation .
Irrespective of seasonal variation in vector abundance, An. funestus s.s., An. gambiae s.s. and An. arabiensis were all-important malaria vectors in the study area . Despite high abundance of An. arabiensis and a higher EIR between 2008 and 2010, An. funestus contributed a relatively higher or equal EIR in 2011 and 2012. Historically, An. funestus has displayed high sporozoite prevalence  similar to that observed in this study and in a recent study conducted in neighbouring villages within the valley (Kaindoa et al., unpublished). This trend of increase in abundance and high sporozoite prevalence of An. funestus has been also observed in Asembo district, western Kenya  and so appears to represent a trend across several regions of East Africa.
The huge increase in potential malaria transmission in 2012 (EIR = 226) coincided with an increase in abundance and sporozoite rates in An. funestus as it did in a neighbouring village in the valley (EIR = 467) (Kaindoa et al., unpublished). The substantial increase in An. funestus and its reduced susceptibility to pyrethroids poses a serious threat that needs attention from vector control stakeholders. A separate study in West Africa also reported a rebound in malaria transmission partly being caused by resistance development in An. gambiae to pyrethroids .
A previous study has shown that despite high coverage and usage of LLINs, a high proportion of mosquitoes still enter houses . Therefore, the increase in An. funestus, particularly in the dry season, is likely to exacerbate the problem. Therefore, new strategies to address resistance and outdoor biting behaviour in the early part of the evening as displayed by An. funestus and An. arabiensis are required. This can be achieved through improving the LLINs; for instance, recent development of nets which can target multiple resistant mosquitoes, Olyset® Plus , and by targeting vectors while outdoors using non-resistant compounds, either through larval source management in the dry season via autodissemination of insect juvenile hormone, e.g., pyriproxyfen [66, 67], or by mosquito sterilization with pyriproxyfen , and killing them with toxic sugar-baited traps , non-chemical electric grid  and odour-baited traps .
This study shows that An. funestus and An. arabiensis are important malaria vectors sustaining malaria transmission, with a substantial increase in An. funestus and drastic reduction in An. gambiae s.s. in the year 2012. Malaria transmission significantly declined from 2008 to 2011 and rebounded in 2012 coinciding with an increased role of An. arabiensis and An. funestus in malaria transmission. Although fully susceptible to deltamethrin, An. arabiensis and An. funestus were found to be resistant and with reduced susceptibility to permethrin pyrethroid used for LLINs, respectively. These findings call for complementary vector control tools, robust vector surveillance systems and an insecticide resistance management plan to complement and preserve the efficacy of LLINs.
The study was funded by the Bill and Melinda Gates Foundation through the Global Health Program (Seattle, USA), Grant number OPP52644 and the Addessium Foundation (Reeuwijk, The Netherlands). We are grateful to the community in the villages of Namwawala and Idete for their participation in the study. We particularly thank our colleagues who helped in field data collection and processing: Japhet Kihonda, Peter Pazia, Daniel Lugiko, Nuru Nchimbi, Josephat Kihonda, Matrida Kideule, Cecilia Mchope, and Monica Mpingwa. We thank Deogratius Roman and Salum Aziz for laboratory sample analysis, and Japhet Kihonda for conducting insecticide resistance susceptibility tests, Nico Govella and William Kisinza for supplying insecticides diagnostic concentrations and providing guidance for bioassay testing.
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