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Escalating pyrethroid resistance in two major malaria vectors Anopheles funestus and Anopheles gambiae (s.l.) in Atatam, Southern Ghana



Aggravation of insecticide resistance in malaria vectors is threatening the efforts to control malaria by reducing the efficacy of insecticide-based interventions hence needs to be closely monitored. This study investigated the intensity of insecticide resistance of two major malaria vectors An. funestus sensu stricto (s.s.) and An. gambiae sensu lato (s.l.) collected in southern Ghana and assessed the bio-efficacy of several long-lasting insecticidal nets (LLINs) against these mosquito populations.


The insecticide susceptibility profiles of Anopheles funestus s.s. and Anopheles gambiae s.l. populations from Obuasi region (Atatam), southern Ghana were characterized and the bio-efficacy of some LLINs was assessed to determine the impact of insecticide resistance on the effectiveness of these tools. Furthermore, molecular markers associated with insecticide resistance in both species were characterized in the F0 and F1 populations using PCR and qPCR methods.


Anopheles funestus s.s. was the predominant species and was resistant to pyrethroids, organochlorine and carbamate insecticides, but fully susceptible to organophosphates. An. gambiae s.l. was resistant to all four insecticide classes. High intensity of resistance to 5 × and 10 × the discriminating concentration (DC) of pyrethroids was observed in both species inducing a considerable loss of efficacy of long-lasting insecticidal nets (LLINs). Temporal expression analysis revealed a massive 12-fold increase in expression of the CYP6P4a cytochrome P450 gene in An. funestus s.s., initially from a fold change of 41 (2014) to 500 (2021). For both species, the expression of candidate genes did not vary according to discriminating doses. An. gambiae s.l. exhibited high frequencies of target-site resistance including Vgsc-1014F (90%) and Ace-1 (50%) while these mutations were absent in An. funestus s.s.


The multiple and high intensity of resistance observed in both malaria vectors highlights the need to implement resistance management strategies and the introduction of new insecticide chemistries.

Peer Review reports


Malaria remains the deadliest vector-borne disease accounting for more than 627,000 deaths annually with half of the world’s population being at risk [1]. There have been intensified malaria control and elimination efforts over the past two decades which have helped to avert about 1.5 billion cases and 7.6 million deaths [1]. However, for the past 5 years, there have been no significant reduction in the number of malaria-related cases worldwide [2]. With this stagnation in progress, the targets outlined by World Health Organization (WHO) in the Global Technical Strategy for Malaria 2016–2030 which aimed at reducing the global malaria burden by 90% by 2030 [3] may not be met.

Vector control interventions based on insecticides have been the cornerstone for malaria control and eliminations efforts as they are the most widely used with more than 2 billion long-lasting insecticide-treated net (LLINs) already distributed across the world ( and over 97 million people protected by indoor residual spray [2]. The efficacy of these control tools is threatened by the development of insecticide resistance in the malaria vectors against the few public health insecticides currently approved by WHO [4]. Insecticide resistance to all four main insecticide classes has been reported across the globe with pyrethroid resistance being widespread [5].

Mosquitoes can become resistant to insecticide through changes in the insecticide target preventing its efficient binding (target-site resistance); increased breakdown and elimination of the insecticide by detoxification enzymes (metabolic resistance); cuticle thickening to reduce insecticide penetration (cuticular resistance). Mosquitoes can also change their behaviour to avoid contact with insecticide-treated surfaces, a mechanism termed behavioural resistance [6]. Various Anopheles species have been identified in Africa and shown to differ in their ability to transmit malaria [7], as well as their ability to survive insecticide exposure [8].

To break the resistance cycle and maintain the efficacy of the current and future insecticides, insecticide resistance management strategies need to be integrated into the National Malaria Control Programmes strategic plans. As such, up-to-date data from resistance surveillance in local malaria vectors are essential in decision-making as insecticide resistance is dynamic.

Malaria remains a major public health issue in Ghana, with Anopheles gambiae and Anopheles funestus being the predominant vectors [8]. While much information is available on the insecticide resistance profile of An. gambiae s.l., very little exists for An. funestus s.s. with most data originating from a gold mining town in southern Ghana, Obuasi [9, 10].

Previous studies characterized the insecticide resistance profile of An. funestus s.s. and reported resistance to dichlorodiphenyltrichlororethane (DDT), permethrin and bendiocarb in 2005 and later in 2014, high resistance to pyrethroids, carbamates and DDT were observed with mortality levels below 50% [10]. Metabolic resistance has been identified as the main mechanism since no mutation in the sodium channel gene associated with the target-site resistance phenotype was found [9]. The glutathione S-transferase GSTe2 and the cytochrome P450s CYP6P9a, CYP6P9b, and CYP6M7 previously implicated in pyrethroid resistance were found to be up-regulated [10]. Furthermore, transcriptional analysis of resistant An. funestus s.s. across Africa revealed that the duplicated CYP6P4a and CYP6P4b are significantly more up-regulated in Ghana [11] but their role in pyrethroid resistance has not yet been validated. Recent studies have reported increased pyrethroid resistance levels in An. funestus s.s. populations of Southern and Eastern Africa with mosquitoes surviving longer insecticide exposure and higher doses of insecticides [12, 13]. These escalations of insecticide resistance are more likely to lead to control failure than standard resistance levels [14] by reducing the efficacy of vector control tools which could lead to a rise in malaria incidence and fatalities. Such insecticide resistance surveillance data are lacking for An. funestus s.s. population from West Africa notably in Ghana. An. gambiae s.l. population from Ghana has shown resistance to all four public health insecticides with high-intensity resistance reported to pyrethroids and carbamates and low resistance intensity to pirimiphos methyl [15].

To fill this gap and assist in resistance management, this study aimed to extensively characterize the insecticide resistance level in An. funestus s.s. and An. gambaie s.l. mosquitoes in the Obuasi area (Atatam) in southern Ghana. In addition, the bio-efficacy of some selected new LLINs against these local mosquito populations was determined and the molecular basis of the resistance escalation was investigated.


Study site and mosquito collection

Indoor blood-fed resting Anopheles mosquitoes were collected in the village of Atatam (06° 17.377″ N, 001° 27.545″ W) located in the Adansi Asokwa District, close to Obuasi municipality of the Ashanti Region (Southern Ghana) Fig. 1. The area experiences a semi-Equatorial climate with an average temperature of about 27 °C and average annual rainfall ranging between 1250 and 1705 nm [16]. Most of the inhabitants are practicing cocoa and subsistent farming. Mosquitoes were collected in July (peak of the major raining season) and October (peak of the minor raining season) 2021.

Fig. 1
figure 1

Map of Ghana showing the geographical location of the collection site Atatam

Verbal consent was obtained from the village chief and house owners before starting the collections. Each collection was planned for 3–5 days, and mosquitoes were aspirated using prokopack electric aspirators. Morphological identification of the collected mosquitoes was done using the morphological keys [17]. An. funestus s.l. and An. gambiae s.l. females were morphologically identified and transferred from the cage into paper cups covered with a net and maintained for 5–7 days until they became fully gravid. The mosquitoes were then forced to lay eggs in 1.5 mL micro-centrifuge tubes and the obtained larvae were reared to adults as previously described [18].

DNA extraction and species identification

One hundred and twenty An funestus s.l. F0 females were dissected into head plus thorax and abdomen, after which genomic DNA was extracted from each part using the LIVAK method [19]. Briefly, DNA was isolated from individual mosquitoes that were homogenized in 100 µl of lysis buffer (composed of 0.5% SDS/0.08 M NaCI/O.16 M sucrose/0.06 M EDTA/O.I2 M Tris-HCI, pH 9) and incubated at 65 °C for 30 min. Four Molar potassium acetate was used to precipitate out the proteins followed by centrifugation. Finally, the DNA was rinsed with ethanol, dried and resuspended in deionized water [19]. The cocktail polymerase chain reaction (PCR) [20] was used to identify the specific member of the funestus group collected. In addition, 65 An. gambiae s.l. were also dissected and molecularly identified using the SINE PCR [21].

Plasmodium infection rates

The bisected mosquito head/thoraxes and abdomens were screened separately for Plasmodium falciparum and Plasmodium ovale, Plasmodium vivax, and Plasmodium malariae (OVM) using the TaqMan assays previously described [22]. Sporozoites or oocyst infections were indicated by positive head plus thorax or abdomen respectively. Positive samples were later validated by nested PCR [23].

World Health Organization insecticide susceptibility assays

Non-blood-fed female F1 An. funestus s.s. and An. gambiae s.l. aged between 3 to 5 days were subjected to WHO tube bioassays [24] to determine the insecticide resistance profile. An. funestus s.s. and An. gambiae s.l. mosquitoes were exposed to discriminating concentration (DC), 5 × DC, and 10 × DC of pyrethroids [type I permethrin (0.75%, 3.75% and 7.5%) and type II deltamethrin (0.05%, 0.25% and 0.5%) and alpha-cypermethrin (0.05%, 0.25% and 0.5%)]; the organochlorine [DDT (4%)]; carbamates [bendiocarb (0.1%) and propoxur (0.1%)]; and organophosphates [pirimiphos methyl (0.25%), fenitrothion (1%) and malathion (5%)]. In each test, at least 100 females divided into four replicates of 20–25 females per tube were exposed per insecticide along with 40–50 mosquitoes (2 replicates) were used as controls and exposed to non-impregnated papers. Mosquitoes were exposed for 1 h, and final mortality was recorded after 24 h post-exposure. The impregnated papers were supplied by the WHO supplier at Universiti Sains Malaysia.

The strength of phenotypic resistance was assessed for insecticides where resistance was confirmed for the standard diagnostic doses and for which 5- and 10-times doses are available. Furthermore, a synergist bioassay with 4% Piperonyl Butoxide (PBO) was carried out to assess the possible contribution of metabolic resistance [24]. When control mortality was between ≥ 5% and ≤ 20%, Abbott’s formula was used to correct the test mortality.

WHO cone test

The bio-efficacy of insecticide-treated bed nets against the An. funesus s.s. and An gambiae s.l. populations from Atatam were assessed using cone assays as recommended by WHO [25] with slight modification. Mosquitoes were exposed to the following standard LLINs [PermaNet 2.0, Interceptor, DuraNet, Olyset, MagNet], PBO nets [PermaNet 3.0, Olyset plus] and novel nets [Royal guard and Interceptor G2]. A piece of untreated net was used as a control. Fifty F1 females aged 3 to 5 days old grouped in 5 replicates were aspirated into plastic cones placed over the treated nets and exposed for 3 min before transferring them into a paper cup. Mosquitoes were provided with 10% sugar solution and knockdown and mortality were scored 1 h and 24 h post-exposure respectively.

Genotyping of resistance markers

The L119F-GSTe2, CYP6P9a, and CYP6P9b mutations previously associated with metabolic resistance to DDT and pyrethroids in An. funestus s.s. were genotyped to identify if these markers are also driving resistance in West Africa (Ghana). The L119F-GSTe2 resistance marker genotyping was performed using the allelic-specific PCR [26] and the CYP6P9a and CYP6P9b markers using the PCR restriction fragment polymorphisms [11, 27]. Furthermore, the GABA receptor RDL A296S and Acetylcholinesterase-1 N485I target site mutations associated with dieldrin and carbamate resistance respectively were also genotyped using the Taqman SNP genotyping assay [26, 28]. The target site mutations L1014F and L1014S kdr (both East and West) are strongly associated with resistance to pyrethroids and DDT [29, 30], as well as the N1575Y suggested to either compensate for deleterious fitness effects of 1014F or confer additional resistance to insecticides were also genotyped [31]. In addition, the Ace-1 G119S resistance mutations were assayed in F0 An. gambiae s.l. mosquitoes using the Taqman technique [22]. The association of these markers with phenotypic resistance was determined by genotyping each marker in exposed F1 mosquitoes both in the survivor and dead groups.

Transcriptional profile of major metabolic resistance genes

Quantitative reverse transcription polymerase chain reaction (qRT-PCR) assay was used to assess the expression profile of detoxification genes previously associated with pyrethroid resistance. This included CYP6P9a, CYP6P9b, GSTe2, CYP9K1, CYP6M7, and CYP6P4a for An. funestus s.s. and CYP6M2, GSTe2, CYP9K1, CYP6P4, CYP6Z1, CYP6P3, CYP4G16, and CYP4G17 for An. gambiae s.l. In addition, the expression of the chemosensory proteins SAP1, SAP2 and SAP3 recently shown to be involved in pyrethroid resistance [32] were also assessed in An. gambiae s.l. The expression profile was compared between An. funestus s.s. F1 resistant to deltamethrin (1x, 5x, and 10x), unexposed and FANG insecticide susceptible laboratory strain while for An. gambiae s.l., F1 resistant to permethrin 1x, unexposed and Kisumu laboratory strain were used. This involved extraction of total RNA from 3 pools of 10 F1 mosquitoes each using the Picopure RNA isolation kit (Arcturus) followed by cDNA synthesis and lastly qPCR [33]. The 2−ΔΔCT method was used to calculate the relative expression [34] and fold changes after normalization with housekeeping genes RSP7 (ribosomal protein S7; VectorBase ID: AFUN007153-RA) and Actin (VectorBase ID: AFUN006819-RA) for An. funestus s.s. while ribosomal protein S7 (AGAP010592) and elongation factor (AGAP005128) were used for An. gambiae s.l. Unpaired Student’s t-test was used to determine whether the difference observed in expression was significant.


Species identification

A total of 603 blood-fed Anopheles mosquitoes were collected in July 2021 with 424 (70.32%) morphologically identified as An. funestus s.l. and 179 (29.68%) identified as An. gambiae s.l. Later in October 2021, 574 blood-fed Anopheles were collected with 267 (46.52%) An. funestus s.l. and 307 (53.48%) An. gambiae s.l. Molecular identification by PCR on a subset of 78 F0 An. funestus s.l. revealed that 81.4% of the samples that amplified (70/86) were An. funestus s.s. with a band at 505 bp in addition to 2 An. Parensis (252 bp) and 1 An. Rivulorum (411 bp). SINE PCR performed on 66 F0 An. gambiae s.l. revealed the presence of 60.61% (40/66) An. gambiae s.s. and 39.39% (26/66) An. coluzzii. Hence An. funestus s.s. was the dominant malaria vector at the beginning of the peak of the major raining season while An. gambiae s.l. dominated at the peak of the minor raining season.

Plasmodium infection rates

The head/thoraxes and abdomen of 120 An. funestus s.s. were screened separately to detect the presence of Plasmodium sporozoites and oocysts, respectively. The proportions of oocyst and sporozoite infections were 10.83% (13/120) and 2.5% (3/120) respectively. For the Oocyst infection, 7.5% (9/120) were identified as P. falciparum and 3.33% (4/120) as either P. ovale, P. vivax, or P. malariae (OVM). On contrary, all the sporozoite infections (3/120) were due to P. falciparum (2.5%). Nested PCR confirmed that (6/9) of the Plasmodium-infected oocyst were P. falciparum and 3/4 of the OVM were due to P. malariae. Regarding the Plasmodium sporozoite infection, 2 out of the 3 detected were confirmed to be due to P. falciparum.

For An. gambiae s.l., 41 samples were dissected into head/thoraxes and abdomen. TaqMan revealed an oocyst infection rate of 14.63% (6/41) with 66.67% due to P. falciparum and 33.33% OVM. A sporozoite infection rate of 9.76% (4/41) due to P. falciparum was obtained. Interestingly, it was also noted that all the Plasmodium infections were recorded in An. gambiae s.s. while no infection was observed in An. coluzzii. Nested PCR recorded no infection from the four sporozoite positive samples detected by TaqMan and revealed similar results with oocyst infection obtained by TaqMan. Also, the nested PCR further identified the 2/41 OVM samples as P. malariae.

Insecticide resistance profile at diagnostic insecticide concentrations

An. funestus s.s. from Atatam were resistant to three classes of insecticides used in public health including pyrethroids [both type I (permethrin) and type II (deltamethrin and alphacypermethrin)], organochlorine (DDT), and carbamates (bendiocarb and propoxur) but fully susceptible to organophosphates (pirimiphos methyl and malathion) at standard diagnostic doses (1X). The lowest mortalities were observed for pyrethroids with mortality rates of 1.25 ± 1.25% for alpha-cypermethrin 1x, 11.6 ± 5% for permethrin 1 × and 5.33 ± 2.37% for deltamethrin 1x. DDT had a lower mortality rate of 43.09 ± 11.34% compared to the carbamates, bendiocarb 1x (66.3 ± 5.18%), and propoxur (83.47 ± 3.81%) (Fig. 2A). On the other hand, An. gambiae s.l. was found resistant to all four main classes of insecticides used in public health. An. gambiae s.l. was highly resistant to pyrethroids and organochloride DDT with mortality ranging from 0–3.7% and 1.25% respectively (Fig. 2B). This An. gambiae s.l. population was also resistant to organophosphates including malathion and fenitrothion with mortality rates of 50 ± 7% and 34.06 ± 7.67% respectively (Fig. 2B) while a possible resistance to pirimiphos methyl with a mortality rate of 91.13 ± 2.64% was observed. The mortality rates for the carbamates, bendiocarb and propoxur were 40.73 ± 2.86% and 45.0 ± 3.10% respectively (Fig. 2B).

Fig. 2
figure 2

Insecticide susceptibility profile of Anopheles species collected in Atatam exposed to 1x, 5 × and 10 × concentrations of insecticides A Percentage mortality of Anopheles funestus 1 × for various insecticides B Percentage mortality of Anopheles gambiae s.l. 1 × for various insecticides C Resistance intensity of Anopheles funestus under 1x, 5 × and 10 × doses. D Resistance intensity of Anopheles gambiae s.l. under 1x, 5 × and 10 × doses

Intensity of resistance to pyrethroids and carbamates

The resistance intensity was determined for the pyrethroids (permethrin, alpha-cypermethrin, and deltamethrin) and the carbamate bendiocarb. An. funestus s.s. population from Atatam were resistant to both 5 × and 10 × doses of permethrin, deltamethrin, and alpha-cypermethrin hence showing a high-intensity resistance with mortality rates below 90% at 10 × doses of 76.35 ± 3.87%, 67.61 ± 12.45% and 45.17 ± 4.54% respectively (Fig. 2C). At 5 × dose, mortality rates were below 50% for deltamethrin (13.68 ± 1.01%), alpha-cypermethrin (43.19 ± 7.1%) while permethrin had a higher mortality rate (58.95 ± 2.95).

An. gambiae s.l. also showed high resistance intensity for the 3 insecticides at higher doses. An. gambiae s.l. was more resistant to type II pyrethroids (alpha-cypermethrin and deltamethrin) than type I pyrethroids (permethrin) with higher mortalities scored with an increase in permethrin concentration (Fig. 2D). Permethrin gave mortality rates of 3.70 ± 0.96% at 1x, 48.99 ± 11.85 at 5 × and 73.71 ± 10.75% at 10 × while alpha-cypermethrin and deltamethrin gave 1.09 ± 1.09% and 0% at 1x; 9.12 ± 3.56% and 9.0 ± 3.8% at 5 × and 19.05 ± 4.31% and 23.00 ± 9.5% at 10x. An increase in bendiocarb dose was associated with a slight increase in mortality from 35.56 ± 2.59% at 1 × to 55.01 ± 2.58% at 5 × and a further 50.02 ± 5.84% at 10 × revealing a high resistance intensity (Fig. 2D).

PBO synergist-insecticide bioassay

A significant recovery of susceptibility was observed when An. funestus s.s. mosquitoes were pre-exposed to the synergist piperonyl butoxide (PBO) before exposure to permethrin 1 × and alpha-cypermethrin 1x. Overall, the recoveries for permethrin and alpha-cypermethrin were 75.66% and 85.95% respectively indicating partial involvement of cytochrome P450 enzymes (Fig. 3A). Inhibition of cytochrome P450 enzymes in An. gambiae s.l. by pre-exposure to PBO before insecticide had a limited impact on the resistance profile. Pre-exposure gave a recovery rate of 11.86% for permethrin, 12.87% for alpha-cypermethrin, 39.20% for deltamethrin, and 23.45% for bendiocarb (Fig. 3B) showing that cytochrome P450s could be playing a minor role in the resistance observed alongside the implication of other enzymes or resistance mechanisms.

Fig. 3
figure 3

PBO Synergist bioassay and cone assay results. A Proportion mortality of Anopheles funestus to pyrethroids when pre-exposed to PBO synergist B Proportion mortality of Anopheles gambiae s.l. to pyrethroids when pre-exposed to PBO synergist C Bio-efficacy of different LLINs An. funestus s.s. mosquitoes from Atatam using WHO cone bioassays D Bio-efficacy of different LLINs against An. gambiae s.l. mosquitoes from Atatam using WHO cone bioassays

Insecticide-treated bed net bio-efficacy

The effectiveness of some LLINs was determined following the WHO guidelines for cone assays. For An. funestus s.s., the assays revealed a loss of efficacy of conventional bed nets (PermaNet 2.0, Interceptor, DuraNet, Olyset, MagNet) with mortalities ranging from 0 to 13.94 ± 1.93% (Fig. 3C). The PBO-based nets were the most effective with mortality rates above 80%. Surprisingly, the novel dual ingredient nets (Royal guard and interceptor G2) had mortality rates below 80% (Fig. 3C).

Similar results were obtained for An. gambiae s.l. with reduced efficacy for conventional bed nets like PermaNet 2.0 (9.83 ± 6.41%), Olyset (23.82 ± 16.93%), DuraNet (0%), Interceptor (13.04 ± 4.90%) and MagNet (1.67 ± 8.27%) (Fig. 3D). Only, PermaNet 3.0 net showed high efficacy with 100% mortality while the other PBO-based net Olyset plus gave low mortality of 32.20 ± 18.07%. The novel nets surprisingly showed a reduced efficacy with mortality below 80%. Interceptor G2 had remarkably low mortality of 6.82 ± 7.03% 72 h post bioassays while Royal Guard scored the second-highest mortality (78.47 ± 8.27%) after PermaNet 3.0 (Fig. 3D). All the Nets used in this study were also tested against the An. gambiae s.s. Kisumu laboratory susceptible strain which resulted in 100% mortalities.

Detection and allelic distribution of insecticide resistance markers in field samples

Genotyping of 53 F0 An. funestus s.s. for both target site and metabolic resistance markers detected resistant genotypes only for A296S-RDL and L119F-GSTe2 while the CYP6P9a, CYP6P9b, and N485I-Ace were completely susceptible. The 296S-RDL resistant allele was present at a high frequency of 84% close to what was reported in 2014 (78.95%) [10]. In terms of genotypes, 72% of the individuals genotyped were RR (36/50), 4% were SS (2/50) and 24% RS (12/50) similar to the frequencies reported in 2014 (Fig. 4A).

Fig. 4
figure 4

Temporal monitoring of percentage frequency of resistance markers and expression profile of candidate genes A A296S mutation associated with resistance to dieldrin and B L119F-GSTe2 mutation associated with DDT/pyrethroid resistance C Frequencies of resistance markers (kdrW-L1014F, N1575Y, Ace-1 G119S, Gste2-I114T) in An. gambiae D Differential expression of candidate resistance genes by qPCR between Deltamethrin 1x, 5 × and 10 × An. funestus s.s. resistant mosquitoes, unexposed relative to FANG susceptible lab strain. E Differential expression of candidate resistance genes by qPCR between permethrin 1x, 5 × and 10 × An.gambiae s.l. resistant mosquitoes, unexposed relative to Kisumu susceptible lab strain

Detection of the L119F-GSTe2 mutations associated with DDT/pyrethroid resistance in 53 F0 non-exposed mosquitoes revealed a similar trend to A296S-RDL with the GSTe2 119F resistance allele present at 53.77%. Genotype distribution detected 30.19% RR (16/53) individuals, 47.17% (25/53) RS and 22.64% SS. Overall the frequencies of the L119F-GSTe2 mutation were similar to those obtained in 2014 both at the allelic and genotypic levels [10] (Fig. 4B).

For An. gambiae s.l., the target-site resistance markers (Kdr-west/Kdr-East, N1575Y, and Ace-1), as well as the metabolic resistance marker (GSTe2 I114T), were genotyped in 38 F0. The 1014F_resistant allele was found at a high frequency (90.79%) while the 1014S resistant allele was absent (Fig. 4C; Additional file 1: Table S1). The N1575Y mutation was completely absent in the subsamples used. The 119S Ace-1 resistant marker associated with resistance to carbamates and organophosphates was detected at 50% and genotypic frequencies of 45.71% (16/35) RR, 8.57% (3/35) RS and 45.71% (16/35) SS. At the species level, the 119S frequency was higher in An. gambiae s.s. 64% versus 13.63% in An. coluzzii (Fig. 4C; Additional file 1: Table S1). Genotyping of the Gste2-I114T showed that the 114 T resistant allele was present at 77.78% with 63.89% (23/36) RR, 27.78% (10/36) RS, and 8.33% (3/36) SS.

Role of L119F-GSTe2 mutations in DDT and escalation of pyrethroid resistance in An. funestus s.s.

Genotyping of the L119F GSTe2 in 38 dead and 43 alive F1 samples exposed to DDT showed that the 119F allele was present at a higher frequency of 76.74% in survivors compared to the dead mosquitoes (31.57%) while the L119 allele was present at 23.26% in the survivors versus 68.42% in the dead mosquitoes (Additional file 1: Table S2). This revealed an association between the 119F mutation and the ability to survive exposure to DDT (OR: 7.02; 95% CI: 3.75–13.16; P < 0.0001) (Fig. 5A, D). A comparison of genotypes also showed a higher frequency of 58.14% (25/43) for the F/F in alive mosquitoes while the L/L were more in the dead samples at 52.63% (20/38) (Additional file 1: Table S2). There were no significant differences in the L/F genotype among the dead (31.58%) or alive (37.20%) groups. The observed association was stronger in the homozygote state than in the heterozygote state (OR: 9.38; 95% CI: 1.85–47.52; P = 0.0069) indicating an additive effect. F/F and F/L genotypes also showed higher association with the survival ability post-exposure to DDT compared to the L/L with odds ratios of 41.67 (95% CI: 7.57–229.21; P < 0.0001) and 13.33 (95% CI: 2.60–68.39; P = 0.0019) respectively.

Fig. 5
figure 5

Association of the L119F GSTe2 mutation with insecticide resistance phenotype. Genotypic frequencies of L119F GSTe2 resistance mutation among F1 An. funestus s.s. mosquitoes exposed to A DDT, B deltametrhin 5x, and C deltamethrin 10x. Allelic frequencies of L119F GSTe2 resistance mutation among F1 An. funestus s.s. mosquitoes exposed to D DDT, E deltamethrin 5X and F) deltamethrin 10x

The contribution of the L119F GSTe2 in the escalation of pyrethroid resistance was checked by genotyping this marker in dead and alive mosquitoes exposed to deltamethrin 1x, 5 × and 10 × concentrations. Due to the low mortality rate of 5.33 ± 2.37% at 1 × with only 3 mosquitoes dead, it was not possible to check the correlation at this dose. Using the 5 × samples showed an association with deltamethrin resistance at this increased dose, with a predominance of the 119F allele (63.24%) among the alive compared to the L119 allele (36.76%) (OR; 2.35; 95% CI: 1.33–4.15; P = 0.0032). Genotypic frequencies showed that all the alive were either F/F (26.47%) or L/F (73.52%) while all the L/L were among the dead (19/43). F/F and L/F genotypes were associated with greater chances of surviving 5 × deltamethrin exposure than the L/L with odd ratios of 26.64 (95% CI: 1.58–555.75; P = 0.0234) and 79.56 (95% CI: 4.43–1428.10) respectively (Fig. 5B, E). Detection of the L119F among the 10X deltamethrin alive and dead samples revealed no clear association of this mutation with the ability to survive exposure to a higher dose as the results obtained were not significant (Fisher exact test: 0.247; P < 0.05) (Fig. 5C, F). The 119F allele was present at a higher frequency in the dead (43.93%) than alive (35.42%) samples while surprisingly the L119 allele was present more in the alive (64.58%) than dead (56.06%) samples but this was at non-significant levels.

Role of G119S Ace-1 mutations in carbamate and organophosphate resistance in An. gambiae s.l.

Eighty-seven (51 alive and 36 dead) F1 An. gambiae s.l. samples were used to check the association between resistance to the carbamate bendiocarb and the G119S mutation in the Ace-1 gene. The 119S resistant allele was found more in the survivors at 88.24% and completely absent in the dead samples (Additional file 1: Table S2). Some samples carrying the G119 susceptible allele (14.28%; 6/42) were able to survive exposure to bendiocarb, but the majority 85.24% (36/42) died after exposure (Fig. 6C). A similar pattern was seen at the genotypic level with only RR and SS genotypes detected at frequencies of 88.24% and 11.76% respectively (Fig. 6A). Hence the resistance to bendiocarb is associated with the presence of the 119S Ace-1 allele (OR; 511; 95% CI: 27.86–9373.55; P < 0.0001).

Fig. 6
figure 6

Association of the Ace-1 G119S mutation with insecticide resistance phenotype. Distribution of Ace-1 G119S resistance mutation genotypes among F1 An. gambiae s.l. mosquitoes exposed to A Bendiocarb, and B pirimiphos methyl. C and D show the allelic distribution of G119S mutation among mosquitoes exposed to C bendiocarb and D pirimiphos methyl

The association between resistance to pirimiphos methyl and the G119S Ace-1 resistance mutation was also investigated using 67 (7 alive and 60 dead) F1 An, gambaie s.l., obtained from bioassays (Fig. 6B, D). TaqMan results identified 31 119S/119S (RR) of which only 7 (22.58%) had survived exposure to pirimiphos methyl while the remaining 24 (77.42%) were dead. All the G119/G119 (SS) were recorded in the dead following the exposure (Additional file 1: Table S2). Hence, the 119S resistant allele was found to be associated with resistance to pirimiphos methyl (OR = 22.35; 95% CI: 1.22–409.47; P < 0.0001).

Transcription profile of resistance genes in An. funestus s.s.

The expression levels of certain candidate genes associated with insecticide resistance were determined. This included the duplicated CYP genes CYP6P4a and CYP6P9a/b, CYP6M7, GSTe2, and CYP9K1 all known to drive pyrethroid resistance in An. funestus s.s. populations across Africa. These genes were up-regulated in the survivors exposed to 1 × deltamethrin compared to the susceptible FANG except for CYP9K1 (Fig. 4D , Additional file 1: Table S3). CYP6P4a was the most up-regulated with a massive fold change of 518.17 ± 51.27 followed by CYP6P9a (12.40 ± 0.71), CYP6P9b (12.61 ± 0.50), CYP6M7 (7.48 ± 0.91), and lastly GSTe2 (6.51 ± 2.7) (Fig. 4D , Additional file 1: Table S3). There was no significant difference observed between the survivors and unexposed (control) indicating that these genes are constitutively expressed except for CYP6P4a (p value = 0.027). Analysis of the expression profile of these genes in samples alive after exposure to 1x, 5 × and 10 × doses showed that higher doses do not have much impact on the expression. Apart from CYP6P4a, a comparison of the actual expression profile to the previous study done in 2015 revealed no major change in the expression of CYP6P9a, CYP6P9b, CYP6M7, and GSTe2 with previous data showing 13.85 ± 0.37; 8.52 ± 0.18; 5.62 ± 0.65 and 13.59 ± 2.53 respectively.

Transcription profile of resistance genes in An. gambiae s.l.

qRT-PCR was used to estimate the expression of 12 candidate genes relative to the Kisumu susceptible laboratory strain. Several genes were found to be upregulated in An. gambiae s.l. population from Atatam. Genes upregulated with a fold change greater than 2 were in the order CYP9K1 > SAP1 > CYP6M2. For the cytochrome P450s, CYP9K1 and CYP6M2 were 10 and 4- folds more expressed than in the susceptible Kisumu respectively. Out of the 3 chemosensory proteins, 2 (SAP1 and SAP2) were found to be up-regulated at around 5 and 2 folds respectively. The cytochrome P450 monooxygenases CYP4G16 and CYP4G17 were downregulated in the survivor mosquitoes. Some genes (CYP6M2, SAP1, and SAP2) were found to be induced as the expression levels were higher in the exposed compared to the non-exposed group (Fig. 4E , Additional file 1: Table S3). Analysis of the level of expression of these genes as the insecticide dose increased from 1 × to 5 × and 10 × revealed no further change in expression level.


Until now the fight against malaria relies mostly on vector control interventions whose effectiveness is threatened by the rise of insecticide resistance. For adequate actions to be taken, it is important to monitor the evolution of insecticide resistance and assess its impact on the effectiveness of current control tools. Knowledge of the susceptibility profile of local malaria vectors against insecticides can guide in designing and implementing suitable resistance management strategies to preserve the efficacy of the current and future vector control tools, especially in malaria-endemic countries. In this study, An. funestus s.s. and An. gambiae s.l. population collected in Southern Ghana showed multiple and high-intensity resistance to most insecticides used in public health. The data from this study provide valuable information for the NMCPs which will help in decision making and better implementation of insecticide resistance management.

Malaria transmission has not abated in Atatam with two major vectors present

An. funestus s.s. was found to be the main malaria vector in Atatam at the time of collection which is in accordance with previous studies carried out in this area [8,9,10]. The role of An. funestus s.s. in malaria transmission was highlighted with a Plasmodium infection rate of 10.8% and 2.5% for the oocyst and sporozoite infection respectively. The oocyst rate was similar to the 12.5% reported in 2014 for whole mosquitoes [10], and the sporozoite rate of 1.81% reported in 2010 [8]. This indicates no reduction in the infection rates notwithstanding the use of bed nets in the area. Despite this, the oocyst infection rate was lower than that reported in other regions across Africa including Cameroon (15%) [35, 36] and Congo (22.2%) [37]. Similarly, the sporozoite Plasmodium infection rate was also lower when compared to those previously report in Nigeria (54.55%) [38], Cameroon (5%) [35, 36], Uganda (4.5%) [13] and Malawi (4.8%) [39]. P. malariae and P. falciparum were both found at the oocyst stage but only P. falciparum was present at the sporozoite stage.

The Plasmodium infection rate in An. gambiae s.l. (14.28%) was higher than that of An. funestus s.s. both at the sporozoite and oocyst rate indicating that both vectors are involved in malaria transmission. This is higher than the infection rate of 4.9 previously reported in Atatam. This was still more than what was observed in other localities in southern Ghana: Tarkwa (4.7%), Ahafo (8.3%), and Akyem (5.03%) [8].

An. gambiae s.l. and An. funestus s.s. both exhibit multiple and aggravated resistance to insecticides

This study also characterized the insecticide susceptibility pattern of An. funestus s.s. and An. gambiae s.l. from Ghana. An. funestus s.s. showed a high level of resistance to pyrethroids and moderate resistance to DDT and carbamates. A comparison of bioassay results done in 2014 and 2021 showed an increase in resistance level for permethrin indicated by reduced mortality rates from 36.11 ± 3.87% in 2014 to 11.6 ± 5% in 2021. An increase in susceptibility was observed for DDT (17.86 ± 4.51% in 2014 to 43.09 ± 11.34% in 2021) and bendiocarb (21.88 ± 10.71% in 2014 to 66.3 ± 5.18% in 2021). The resistance level has increased when compared to previous reports, especially for the pyrethroids where mortality rates ranged from 1.25 ± 1.25 to 11.67 ± 5% which is quite concerning as the main vector control tool in Atatam is alpha-cypermethrin impregnated LLINs (MagNet) distributed during the last campaign. Intensity bioassays showed that An. funestus s.s. can withstand 5 × and 10 × doses of permethrin, alpha-cypermethrin, and deltamethrin with more than 20% of mosquitoes alive at 10X. This resistance intensity profile is higher than that recently reported in other populations from Eastern Africa [40]. Pre-exposure to PBO synergist greatly increased the efficacy of pyrethroids hence revealing the implication of metabolic resistance more precisely the cytochrome P450s detoxification enzymes. The implication of cytochrome P450s implies that LLINs with PBO could be more effective than the conventional bed nets with insecticides only. This was in line with the cone assays results which tested the bio-efficacy of some commercially available nets against this An. funestus s.s. population and revealed that PBO-based bed nets were the most effective even surpassing the novel bed nets (Royal guards and interceptor G2). PBO-based bed nets have been shown to reduce malaria incidence [41] and increase personal protection [42] in areas with pyrethroid resistance. The full susceptibility to organophosphates indicates that IRS with pirimiphos methyl (Actellic 300CS) could also be an option in curbing pyrethroid resistance in this area as previously shown in northern Ghana [43] and western Kenya [44]. Even though a reduced performance of conventional bed nets was observed with cone assays, more studies using either experimental hut or looking at the delayed mortality are needed to assess the impact of such multiple resistance on the effectiveness of insecticide-based interventions.

An. gambiae s.l. was highly resistant to all public health insecticides tested with possible resistance to pirimiphos methyl. The mortality due to pyrethroids was extremely low similar to what has been reported in other localities in Ghana [15] and other countries such as Ivory Coast [45], Cameroon [46], Nigeria [47] and Democratic Republic of Congo [48]. The intensity of pyrethroid resistance was higher for type II which is different from the frequent pattern where An. gambiae s.l. is often more resistant to type I than type II as observed elsewhere [46] but similar to the results reported by Pwalia et al., in 2017. The intensity of resistance to bendiocarb was also high even at 10 × showing that this population is exhibiting both high intensity and multiple resistance. Synergist assays using PBO indicated the involvement of cytochrome P45Os but with a low recovery rate suggesting that other mechanisms might be involved. The recovery rate with PBO was lower than those previously reported by [15] and [49] who evaluated the synergizing effect of PBO in enhancing the efficacy of pyrethroids. The impact of the multiple and high intensity of resistance of An. gambiae s.l. from Atatam on the bio-efficacy of different nets was assessed through cone assays and revealed low mortality, particularly for pyrethroid-only bed nets. This low efficacy of pyrethroid only nets has been reported across Africa by several authors [15, 37]. Pyrethroid-PBO net (PermaNet 3.0) was the most effective suggesting that Pyrethroid-PBO nets could better help in controlling malaria in this region. Epidemiological studies and semi-field trials carried out in Africa have shown that these Pyrethroid-PBO nets provide more protective capacity than pyrethroid-only nets in areas with high intensity of resistance [41, 42, 50].

Previous studies have reported the absence of target-site resistance in An. funestus s.s. both in Ghana [9] and across Africa [51]. PBO synergist bioassays result established the involvement of cytochrome P450s with CYP6P4a, CYP6P9a, CYP6P9b and CYP6M7 genes being up-regulated. CYP6P9a/b were up-regulated but the expression levels were lower than those reported in Mozambique, southern Africa [12]. The previously identified candidate gene CYP6P4a was highly overexpressed at about 12 times higher than what was reported in 2015 by Weedall et al. (2019). Further studies are needed to characterize the role of this gene in insecticide resistance to allow the development of a diagnostic tool to track insecticide resistance in this region. Genotyping for the molecular markers previously identified in the promoters of CYP6P9a and CYP6P9b genes showed that these samples are susceptible indicating that other mechanisms such as trans-regulatory factors, different from those in southern Africa may be involved. The GSTe2 was found to be up-regulated (FC: 6.51 ± 2.7) and the 119F mutation was also found at a high frequency which correlated strongly with DDT resistance. The significant correlation between the 119F_GSte2 allele and the ability to survive exposure to 5 × deltamethrin is an indication that GSTe2 contributes to resistance escalation but the lack of correlation at 10 × could suggest that other molecular factors are driving a higher level of resistance. Overall, the frequency of GSTe2 in Atatam is higher than reported in Cameroon (23%) [36, 52], Uganda (10%) [13] and Mozambique (7%) [12]. But lower than the 100% reported in Benin [53]. The frequency of A296S mutation associated with resistance to dieldrin remained constant (80%) even with the discontinued use of dieldrin similar to what is observed in An. gambiae [54] thereby posing a limitation on the use of other cyclodienes in vector control. The widespread pyrethroid resistance has led to the development of new LLINs which contain the pyrethroid combined with other chemicals such as PBO, chlorfenapyr or pyriproxyfen. Low mortality was obtained with interceptor G2 but further studies using the WHO tunnel test are needed to confirm its effectiveness as cone assays are not a reliable method to measure the bioefficacy of the chlorfenapyr component [55].

In An. gambiae s.l., the vgsc-L1014F mutation associated with pyrethroid and DDT resistance was very high at a frequency of 91.4% approaching fixation like in other localities across Africa which could explain the very high pyrethroid resistance observed in Atatam. The Ace-1 119S point mutation characterizing resistance to carbamates and organophosphates was found at a moderate frequency of 50% lower than the 76% frequency previously reported in Accra [15]. Genotyping of this mutation in F1 survivors and dead mosquitoes exposed to bendiocarb and pirimiphos methyl confirmed the link between this mutation and resistance with the 119S being strongly associated with resistance to Bendiocarb (OR; 511; 95% CI: 27.86–9373.55; P < 0.0001) than with pirimiphos methyl (OR; 22.35; 95% CI: 1.22–409.47; P < 0.0001). Grau-Bove et al. (2021) recently showed that pirimiphos methyl resistance is due to a combination of the G119S non-synonymous mutation and copy number variation (CNV) in the acetylcholinesterase Ace-1 gene. Unfortunately, the involvement of CNV was not investigated here. The high frequency of the 119S mutation in An. gambiae s.s. (64%) compared to An. coluzzii could be explained by the fact that Ace-1 substitution evolved in An. gambiae s.s. before introgressing in An. coluzzii as suggested by [56]. qRT-PCR results also revealed the overexpression of multiple detoxification genes (CYP9K1, CYP6M2 and CYP6P4) which have also been found up-regulated in resistant mosquitoes from the Ivory Coast [57]. In addition, the sensory appendage proteins SAP1 and SAP2 previously shown to be overexpressed in West Africa and to also have a high-affinity binding to pyrethroids were found to be upregulated in this population. The lower expression of cytochrome P450s observed in An. gambiae s.l. compared to An. funestus s.s. further supports the contrasting resistance mechanisms in these two species and supports the lack of recovery after PBO exposure in An. gambiae. This reveals the complexity of insecticide resistance phenotype which involves a combination of multiple mechanisms.

In both species, the link between increased overexpression of known detoxification genes and high pyrethroid resistance was investigated with no differences observed between 1x, 5x, and 10 × correlating with previous results in An. funestus s.s. from Uganda [13] but different from what has been reported in An. coluzzii from Burkina Faso [58]. This lack in difference could be due to the fixation of resistance mechanisms in field populations due to the strong selective pressure exerted by high bed net coverage [59]. In addition, the frequencies of resistance markers were also determined with no association observed at higher doses. This is a narrow approach that does not take into account the contribution of other genes and target site resistance. Taking all these into account, there can be other factors that need to be investigated to understand the drivers of resistance escalation such as the contribution of other detoxification genes, target site, sequestration, cuticular resistance, or microbiome. Hence high-throughput techniques such as RNA-sequencing or whole genome sequencing could facilitate the identification of the molecular drivers contributing to high-intensity resistance.


The high and multiple insecticide resistance in An. funestus s.s. and An. gambiae s.l. reported here represents a serious threat to the fight against malaria in Ghana and calls for action to implement insecticide resistance management strategies. The susceptibility to organophosphates and recovery with PBO suggests that vector control tools with this insecticide class could be more appropriate in this area. Ultimately, future vector control interventions should rely on novel insecticide ingredients other than pyrethroids to mitigate the adverse impact of this escalating and multiple resistance in the major malaria vectors.

Availability of data and materials

All data generated or analysed during this study are included in this published article and its Additional files.


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We are thankful to the AngloGold Ashanti Malaria Control (AGAMal) team for allowing us to use their insectary and assisting us with the field collections.


This research was funded by the Bill and Melinda Gates Foundation (INV-006003 to CSW) and a Wellcome Trust Senior Research Fellowship grant to CSW (217188/Z/19/Z). For the purpose of open access, the authors have applied a CC BY public copyright license to any Author Accepted Manuscript version arising from this submission.

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C. S. W. designed the research, C.S.W, M.M.J.L., M.O, G.A and E.K.N supervised the fieldwork. M.M.J.L, M.T, B.D.M and T.T.A performed the insecticide susceptibility and cone assays, M. T., F. N. N., M. J. W. performed the molecular analyses. M.M.J.L. and C.S.W wrote the manuscript with contributions from all the authors. All authors read and approved the final version of the manuscript.

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Correspondence to Leon M. J. Mugenzi or Charles S. Wondji.

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Additional file 1

: Table S1. Frequency of target site mutations characterized in Anopheles gambiae (s.l.) F0 from Atatam. Table S2. Frequency of L119F-GSTe2 resistance markers among dead and alive An. funestus exposed to DDT, deltamethrin 1x, 5x and 10x. Table S3. Differential expression of metabolic resistance genes among F1 Deltamethrin 1X, 5x, 10x and unexposed mosquitoes from Atatam compared with the FANG susceptible strain. Table S4. Differential expression of metabolic and cuticular resistance genes among the An. gambiae sl population from Atatam as compared with the Kisumu susceptible strain.

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Mugenzi, L.M.J., Akosah-Brempong, G., Tchouakui, M. et al. Escalating pyrethroid resistance in two major malaria vectors Anopheles funestus and Anopheles gambiae (s.l.) in Atatam, Southern Ghana. BMC Infect Dis 22, 799 (2022).

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  • Insecticide resistance
  • Atatam
  • Anopheles
  • Malaria
  • Long-lasting insecticidal nets