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Diversity and transmission competence in lymphatic filariasis vectors in West Africa, and the implications for accelerated elimination of Anopheles-transmitted filariasis
Parasites & Vectors volume 5, Article number: 259 (2012)
Lymphatic Filariasis (LF) is targeted for elimination by the Global Programme for the Elimination of Lymphatic Filariasis (GPELF). The strategy adopted is based on the density dependent phenomenon of Facilitation, which hypothesizes that in an area where the vector species transmitting Wuchereria bancrofti are Anopheles mosquitoes, it is feasible to eliminate LF using Mass Drug Administration (MDA) because of the inability of Anopheles species to transmit low-density microfilaraemia. Even though earlier studies have shown Anopheles species can exhibit the process of Facilitation in West Africa, observations point towards the process of Limitation in certain areas, in which case vector control is recommended. Studies on Anopheles species in West Africa have also shown genetic differentiation, cryptic taxa and speciation, insecticide resistance and the existence of molecular and chromosomal forms, all of which could influence the vectorial capacity of the mosquitoes and ultimately the elimination goal. This paper outlines the uniqueness of LF vectors in West Africa and the challenges it poses to the 2020 elimination goal, based on the current MDA strategies.
The January 2012 London declaration on neglected tropical diseases (NTDs)  instilled renewed confidence in the global efforts to control or eliminate several NTDs, including lymphatic filariasis (LF). LF, is caused by the filarial parasites Wuchereria bancrofti, Brugia malayi or Brugia timori and is presently endemic in 72 countries . Mosquito species belonging to the Anopheles, Culex, Aedes, Mansonia, Coquillettidia and Ochlerotatus genera are carriers of the LF parasites. In West Africa, Anopheles mosquitoes (vectors of malaria) are the main vectors of LF [3, 4]. Although Culex mosquitoes have been suggested as vectors of LF [5, 6], the data was insufficient to confirm that assertion. As such, there is minimal evidence that Culex mosquitoes contribute to the transmission of the disease. Current practices in the management of LF have been influenced by the push for integrated control of NTDs amenable to mass drug administration (MDA)  and the impact of vector control on LF transmission . MDA coverage for LF increased from three million people treated in 12 countries in 2000, to more than 450 million in 53 countries in 2010 . During that period, the disease was eliminated in China and Korea. Nine countries no longer require MDA  because of a natural decline in transmission intensity attributed to a range/ or multiple factors including vector control, provision of safe water, sanitation and hygiene. Vector control is now among the five strategies recommended by the WHO for prevention, control, elimination and eradication of NTDs in its 2012 road map for implementation . Prior to 2012, the WHO strategy for LF elimination was based primarily on chemotherapy. However, the impact of vector control on LF transmission is becoming increasingly recognised [8, 12–14]. Understanding the roles of different vectors in LF transmission and the implications for accelerated interruption of transmission in West Africa where the LF vectors are also targeted through malaria control efforts is important.
LF control based on density dependent processes in the vectors
The Global Programme for the Elimination of Lymphatic Filariasis (GPELF) strategy is based on the mass drug administration (MDA) with Albendazole and either DEC or Ivermectin to reduce circulating microfilariae (mfs) below a threshold level, to break transmission by the disease vectors. The rationale supporting this strategy is based on results of research on vector-parasite systems that determine whether vectors will be effective in picking up and transmitting infection at low microfilaraemia levels . These vector-parasite combinations are described under the density-dependent processes of “Facilitation” and “Limitation” . Facilitation is the process where, below a certain threshold level of mfs, designated as Webber’s Critical Point , the transmission by anopheline vectors will be interrupted [18–20]. Limitation on the other hand represents a process whereby even at low mf levels there is stable transmission, which is found among culicines [4, 21]. There is, however, a third case of non-regulated transmission by vectors, termed “Proportionality”. In this case, there is a constant percentage (linear relationship) of mf ingested by the vector during a blood meal developing to the infective stage. Limitation and Facilitation in vectors cause deviations from this linear relationship .
Limitation processes are linked with the fact that the number of parasites per mosquito cannot increase indefinitely. The relationship between mf intake and L3 output is linear at the onset and approaches a constant value or might decrease with increasing mf intake, as a result of excess mortality of vectors caused by ingestion of too many mf [21, 22]. Thus in Limitation, there is a maximum threshold below which the limited process is ‘overefficient’ and above which it is ‘under-efficient’ . This relationship has been observed in the culicines [4, 18] which are believed not to be vectors of LF in West Africa, with the possible exception of Mansonia sp., recently reported to harbor infective mf in Ghana . Thus in Limitation, the eradicability of LF is greatly impaired by shifting transmission thresholds towards lower values, requiring higher control efforts.
Facilitation processes on the other hand have been observed in anopheline mosquitoes [18, 19], which are the vectors of LF in West Africa. Blood containing mf moves through the proboscis by a pumping action created by the cibarial and pharyngeal pumps. In some mosquito species, the pumps are lined with denticulate structures (cibarial armature) that can fatally damage passing mf . At low mf densities, this cibarial armature substantially reduces the proportion of surviving mf. However, at high mf densities, the cibarial armature becomes inefficient because it is masked by a few mf promoting the survival of the others. Thus, at high mf densities transmission becomes efficient by shifting transmission thresholds towards higher values, which can more easily be achieved by control measures .
The assumption that it will be easy to use MDA alone in areas where W. bancrofti is transmitted by Anopheles species, including most endemic areas in Africa, was supported by results in Papua New Guinea (PNG), which showed that transmission by An. punctulatus was virtually eliminated after one year of treatment, even though the frequency of carriers in the human population ranged from 10.5% - 52.7% . Also, one of the earliest documented cases of the elimination of LF occurred when indoor residual spraying with DDT to control malaria inadvertently eradicated LF in the Solomon Islands; here also the vector was an anopheline, An. farauti[17, 21]. In contrast, in the Polynesian Islands of Moorea and Maupiti, where the vector was Aedes polynesiensis, over 50 years of MDA using DEC did not eliminate LF . Despite these evidences and the assumption of vector-parasite phenomenon of Facilitation in Anopheles, there is current growing evidence that in certain areas, Anopheles species may be exhibiting the process of Limitation [26, 27].
Diversity of An. gambiae vectors of LF in West Africa
There is diversity among the vectors of LF, and therefore, it may not be practical to generalize based on data from PNG and the Solomon Islands. Threshold levels of microfilaraemia needed for the elimination of anopheline transmitted W. bancrofti LF might differ from species to species. The major Anopheles vectors of LF in West Africa are An. gambiae s.l, and the An. funestus group . These species complexes are made up of distinct species, which are morphologically indistinguishable and may occur in sympatric situations. For example, in Ghana, several sympatric Anopheles species are vectors [26, 28, 29], and these are likely to differ in their vectorial role and in their capacity to transmit low-density microfilaraemia. Results of earlier studies in sub-Saharan Africa on the quantitative relations of transmission intensity and microfilarial reservoir have been found to vary among members of the An. gambiae complex and An. funestus[30–32]. These variations may include the proportion of mfs ingested by Anopheles mosquitoes which are damaged by their cibarial teeth, the percentage of mosquitoes ingesting mf and host mf density and the percentage of mosquitoes infected or mf density per mosquito and numbers of mf per ml of host blood. In their paper that examined the epidemiological significance of these processes, Southgate and Bryan reported the presence of Facilitation in An. gambiae/W. bancrofti from The Gambia, Burkina Faso and Tanzania . In the same paper, although Facilitation was indicated for An. arabiensis/W. bancrofti when data from The Gambia and Tanzania were combined, the results from Tanzania alone did not indicate Facilitation. This difference in results was attributed to the low numbers of mosquitoes studied. Similarly, the observed non-facilitation for An. melas, An. merus and An. funestus was also attributed to low numbers of mosquitoes examined. However, it is possible that the non-Facilitation observed for these Anopheles/W. bancrofti combinations could have been due to variation in transmission efficiency inherent in the vectors and not necessarily to the low numbers of mosquitoes dissected. Webber commented on the possibility of eradicating anopheline-transmitted filariasis but did not discuss the information on An. melas, An. merus and An. funestus as vectors in Africa . Recent studies by Amuzu and colleagues (2010), aimed at examining the cibarial armature of An. gambiae M and S molecular forms and An. melas in an area endemic for LF in Ghana, showed significantly less number of cibarial teeth in the An. melas compared to the M and S forms of the An. gambiae s.s . As such, it is very clear from the above that anopheline LF vectors in West Africa may differ in their capacity to sustain low-level microfilaraemia. Furthermore, in areas of Ghana where MDA has not been able to eliminate transmission after more than 7 years of intervention, the main vector is An. melas (Boakye unpublished reports to WHO).
The diversity in Anopheles vectors of LF in West Africa is well documented from studies of malaria vectors in this region. Five chromosomal forms namely; “Forest”, “Bissau”, “Bamako”, “Mopti” and “Savannah” have been described [33–35]. The Mopti form of An. gambiae s.s, for example, is believed to be more associated with W. bancrofti, and is a relatively poor vector of malaria compared with other species such as the Savannah form [37, 38]. There is further evidence suggesting that cryptic taxa may exist within An. gambiae s.s due to observed inversions in the micromorphology of the second chromosome for different populations  and thus selective effects due to the increase in certain inversion arrangements may result [33–35]. To add to these, incipient speciation has been reported among members of the Anopheles species in West Africa [40, 41], raising further questions as to why these are only reported in West Africa and not elsewhere on the continent [42, 43].
Two widespread molecular types, termed M and S forms [40, 44] have also been described among the Anopheles gambiae s.s. Recent evidence also suggests the existence of two distinct chromosomal forms within the M form . In Mali and Burkina Faso, the M form corresponds to the Mopti chromosomal form, whereas sympatric populations of Savannah and Bamako belong to the S molecular form. However, the correspondence between chromosomal and molecular forms does not hold true elsewhere in West Africa, especially where the Forest chromosomal forms exist [40, 46].
Insecticide resistance has also been reported among the various vectors of LF on the African continent. The pyrethroid resistance mechanism of kdr mutation had been found distributed in the M and S forms of An. gambiae s.s., [47–49]. DDT and pyrethroid resistance have been widely observed in Africa, in An. gambiae s.s. and An. arabiensis, with multiple-resistance mechanisms observed in West Africa [50–53]. These resistance mechanisms may inadvertently influence the density dependent processes and the vector competence of various Anopheles species. Studies have suggested that highly elevated esterases involved in insecticide-resistance may inhibit development of mf in Culex, and similar effects could occur in insecticide resistant Anopheles[55, 56].
The variability in diversity of Anopheles vectors of LF in West Africa may also be influenced by climate effects, such as temperature and rainfall, which indirectly may influence the transmission of LF [56, 57]. In a study to assess the environmental factors affecting the distribution of An. gambiae s.s. in Ghana and the effects on disease distribution, de Souza and colleagues noted that temperature was the key factor affecting the distribution of the M and S forms of the An. gambiae s.s and that the M was significantly correlated with LF, and more prevalent in the high LF areas compared to low LF areas . West Africa is the only region with the highest number of ecological zones (Mangrove, Coastal Savannah, Guinea Savannah, Sudan Savannah, Sahel Savannah, Semi-deciduous Forest and Evergreen Forest) in the world, the impact of these ecologies on vector diversity and disease transmission dynamics should not be overlooked. As such, the climate impacts on the biology of disease vectors will greatly affect their importance. Thus, an understanding of biodiversity and the importance of vector ecology crucial for the successful control of vector diseases [56, 57].
Eradicability of lymphatic filariasis in West Africa
A single strategy of MDA has been advocated for the elimination of LF in Africa, notwithstanding the diversity in the vectors of the disease. Some evidence [59, 60] suggests the need for vector control as a supplement to MDA, in some areas, to achieve the elimination target of GPELF. For this, an appropriate vector control strategy to complement MDA in Africa will have to take a cue from previous malaria control efforts [61, 62]. Historically, success in combating malaria has been attributed to mosquito control; yet, in recent times, this strategy has largely failed due to various reasons, including the development of insecticide resistance , economic Limitations and gaps in the basic biological knowledge of these vectors .
Vector control is an important component of the control of vector-borne diseases. Early efforts, before the era of DDT to control pests and disease vectors, took an ecological approach in the form of physical modification of the environment, chemical control and personal protection . After the introduction of DDT and the synthetic insecticides, this approach lost its prominence and vector control became synonymous with insecticide use. The use of DDT and its analogs was heralded as the solution for the control of all insect pests, including vectors of human infection. This led to improper insecticide use, which had an enormous negative impact on non-target organisms causing a loss of biodiversity. Although most of the negative impacts resulted from insecticide application to control agricultural pests, vector control suffered as a consequence. This situation coupled with the development of vector resistance to most insecticides, and the high cost of new insecticides and their application led to a loss of interest in vector control and put emphasis on chemotherapy .
The GPELF is based on a strategy of MDA with Albendazole and DEC or Ivermectin, with the aim of reducing the parasite load in the human host, thereby preventing transmission, and a target of 80% coverage of the population at risk for at least 5 years  has been proposed. This ideal is not always achievable because of programmatic issues of drug distribution  and the perpetual threat of drug resistance [68, 69]. Even if this level of coverage is achieved, the diversity of vectors and their differing abilities to transmit low level parasitaemia, may lead to a failure to stop transmission in some regions, after the interruption of MDA. In view of the above, vector control is now considered an important and integral part necessary to achieve elimination in specific areas where MDA alone will not provide the solution. This is especially important, with the very recent report of Mansonia spp. being very efficient vectors of LF, in Ghanaian communities , where they were previously thought to be non-vector species.
Furthermore, studies have suggested differing LF transmission efficiencies for the M and S molecular forms of the An. gambiae s.s [27, 36], with the M form being a more efficient vector. Similar observations have been made with An. melas (Boakye et al., Unpublished), where An. melas is a more efficient vector than the An. gambiae s.s. Based on these findings we propose a model for the interruption of LF transmission in these different vector areas. Thus, areas with the predominant S form may require fewer MDA treatments. With the M form and An. melas exhibiting possible Limitation  areas with the predominant M form and An. melas may require longer treatment periods in addition to vector control measures. The implication of this, should it be tested and proven, will be in its economic importance. As such, in areas where there are high proportions of the An. gambiae S form, LF transmission may be interrupted using 3 to 5 rounds of MDA alone. On the other hand, LF transmission may require more than 5 rounds of MDA, and be complemented with vector control measures in areas with high numbers of An. gambiae M form and An. melas. Areas with equal proportions of M and S forms may also require additional vector control measures. This model, however, needs to be tested and evaluated in different vector areas. Countries like Guinea and Liberia that are yet to start MDA may provide the best settings for testing this model.
In the areas where vector control needs to be implemented, an integrated vector management (IVM) strategy targeted at the major vectors may needs to be adhered to and coordinated with MDA to give the best results at least cost . LF fortunately shares the same vectors with malaria in most African countries and the practices for controlling the vectors of malarial parasites (the use of insecticide treated bednets, indoor-residual spraying) for personal and community protection - can at the same time be effective against both malaria and LF [70, 71]. Even though the GPELF is based on MDA, vector control activities of the 'Roll Back Malaria’ campaign can considerably suppress the risk of W. bancrofti transmission in co-endemic areas.
The use of current MDA alone campaigns, for LF elimination, in West Africa is based on two assumptions; 1. Anopheles species are the only vectors of LF in West Africa and 2. Anopheles vectors of W. bancrofti exhibit the vector-parasite process of Facilitation, based on which elimination is feasible through MDA alone. However, the recognition of different LF vectors in West Africa , with differing vector-parasite processes [26, 27] and differing transmission efficiencies [27, 36], all represent significant challenges to the GPELF 2020 objectives in the West African sub-region. Moreover, despite 5–8 rounds of MDA treatment, field reports have revealed persistent residual LF infections in some communities in Ghana and Burkina Faso . Though reasons of non-compliance could be attributed to these residual infections , others have also hypothesized the influence by vector species [26, 27]. It is also important to note that these observations may not be the same for every West African country, as factors such as ecology, species composition/diversity and insecticide resistance may influence vector transmission potential in different areas. Thus, an understanding of the vector competence of mosquitoes infected with W. bancrofti in different areas would be of particular interest and could be addressed using field or laboratory models. Nonetheless, despite these challenges, LF control efforts in West Africa should be supplemented with vector control, if the GPELF elimination goals of 2020 are to be achieved in West African countries.
Uniting to combat Neglected Tropical Diseases: London Declaration on Neglected Tropical Diseases.http://unitingtocombatntds.org/downloads/press/ntd_event_london_declaration_on_ntds.pdf,
World Health Organization: Fact Sheet No 102. Lymphatic Filariasis. 2012
Appawu MA, Dadzie SK, Wilmot-Baffoe A, Wilson MD: Lymphatic Filariasis in Ghana: Entomological investigation of transmission dynamics and intensity in communities served by irrigation systems in the Upper East Region of Ghana. Trop Med Int Health. 2001, 6: 511-516. 10.1046/j.1365-3156.2001.00737.x.
Subramanian S, Krishnamoorthy K, Ramaiah KD, Habbema JDF, Das PK, Plaisier AP: The relationship between microfilarial load in the human host and uptake and development of Wuchereria bancrofti microfilariae by Culex quinquefasciatus: a study under natural conditions. Parasitology. 1998, 116: 243-255. 10.1017/S0031182097002254.
Agi PI, Ebenezer A: Observations on Filarial Infection in Amassoma Community in the Niger Delta, Nigeria. J Appl Sci Environ Manage. 2009, 13 (1): 15-19.
Anosike JC, Nwoke BE, Ajayi EG, Onwuliri CO, Okoro OU, Oku EE, Asor JE, Amajuoyi OU, Ikpeama CA, Ogbusu FI: Lymphatic filariasis among the Ezza people of Ebonyi State, Eastern Nigeria. Ann Agric Environ Med. 2005, 12: 181-186.
Gyapong J, Gyapong M, Yellu M, Anakwah K, Amofah G, Bockarie M, Adjei S: Integration of control of neglected tropical diseases into health-care systems: challenges and opportunities. Lancet. 2010, 375 (9709): 160-165. 10.1016/S0140-6736(09)61249-6.
Bockarie M, Pedersen E, White G, Michael E: Role of Vector Control in the Global Program to Eliminate Lymphatic Filariasis. Ann Rev Entomol. 2009, 54: 469-487. 10.1146/annurev.ento.54.110807.090626.
Addiss D, The Global Alliance to Eliminate Lymphatic Filariasis: The 6th Meeting of the Global Alliance to Eliminate Lymphatic Filariasis: A half-time review of lymphatic filariasis elimination and its integration with the control of other neglected tropical diseases. Parasit Vectors. 2010, 3: 100-10.1186/1756-3305-3-100.
World Health Organization: Global Programme to Eliminate Lymphatic Filariasis: progress report on mass drug administration. Wkly Epidemiol Rec. 2011, 86: 377-388.
World Health Organization: Accelerating work to overcome the global impact of neglected tropical diseases - A roadmap for implementation. 2012, Geneva-Switzerland: World Health Organization
Ottesen EA: Lymphatic filariasis: Treatment, control and elimination. Adv Parasitol. 2006, 61: 395-441.
Bockarie M, Molyneux D: The end of lymphatic filariasis?. BMJ. 2009, 338: 1686-10.1136/bmj.b1686.
World Health Organization: WHO position statement on integrated vector management to control malaria and lymphatic filariasis. Wkly Epidemiol Rec. 2011, 86: 581-588.
Gyapong JO, Kumaraswami V, Biswas G, Ottesen EA: Treatment strategies underpinning the global programme to eliminate lymphatic filariasis. Expert Opin Pharmacother. 2005, 6: 179-200. 10.1517/146565184.108.40.206.
Brengues J, Bain O: Passages de microfilaires vers l’hémocèle du vecteur, dans les couples Wuchereria bancrofti - Anopheles gambiae, W. bancrofti - Aedes aegypti et Setaria labiatopapillosa - A. aegypti. Cahiers ORSTOM, Série d’Entomolgie Mèdicale et Parasitologie. 1972, 10: 235-249.
Pichon G: Limitation and facilitation in the vectors and other aspects of the dynamics of filarial transmission: the need for vector control against Anopheles transmitted filariasis. Ann Trop Med Parasitol. 2002, 96 (Suppl 2): S143-S152.
Pichon G, Perault G, Laigret J: Rendement parasitaire chez les vecteurs de filarioses. Bull World Health Organ. 1974, 51: 517-524.
Southgate BA, Bryan JH: Factors affecting transmission of Wuchereria bancrofti by anopheline mosquitoes. 4. Facilitation, limitation, proportionality and their epidemiological significance. Trans Roy Soc Trop Med Hyg. 1992, 86: 523-530. 10.1016/0035-9203(92)90096-U.
Webber RH: Can anopheline-transmitted filariasis be eradicated?. J Trop Med Hyg. 1991, 94: 241-244.
Duerr HP, Dietz K, Eichner M: Determinants of the eradicability of filarial infections: a conceptual approach. Trends Parasitol. 2005, 21: 88-96. 10.1016/j.pt.2004.11.011.
Dietz K: The population dynamics of onchocerciasis. The Population Dynamics of Infectious Diseases: Theory and Applications. Edited by: Anderson RM. 1982, London: Chapman & Hall, 209-241.
Ughasi J, Bekhard H, Coulibaly M, Adabie-Gomez D, Gyapong J, Appawu M, Wilson M, Boakye D: Mansonia africana and Mansonia uniformis are vectors in the transmission of Wuchereria bancrofti lymphatic filariasis in Ghana. Parasit Vectors. 2012, 5: 89-10.1186/1756-3305-5-89.
McGreevy PB, Bryan JH, Oothuman P, Kolstrup N: The lethal effects of the cibarial and pharyngeal armatures of mosquitoes on microfilariae. Trans Roy Soc Trop Med Hyg. 1978, 72: 361-368. 10.1016/0035-9203(78)90128-1.
Bockarie MJ, Alexander NDE, Hyun P, Dimber Z, Bockarie F, Alpers MP, Kazura JW: Randomised Community-Based Trial of Annual Single-Dose Diethylcarbamazine With or Without Ivermectin Against Wuchereria bancrofti Infection in Human Beings and Mosquitoes. Lancet. 1998, 351: 162-168. 10.1016/S0140-6736(97)07081-5.
Boakye D, Wilson M, Appawu M, Gyapong J: Vector competence, for Wuchereria bancrofti, of the Anopheles populations in the Bongo district of Ghana. Ann Trop Med Parasitol. 2004, 98 (5): 501-508. 10.1179/000349804225003514.
Amuzu H, Wilson M, Boakye D: Studies of Anopheles gambiae s.l (Diptera: Culicidae) exhibiting different vectorial capacities in lymphatic filariasis transmission in the Gomoa district, Ghana. Parasit Vectors. 2010, 3 (1): 85-10.1186/1756-3305-3-85.
Appawu MA, Baffoe-Wilmot A, Afari EA, Dunyo SK, Koram KA, Nkrumah FK: Malaria vector studies in two ecological zones in southern Ghana. Afr Entomol. 2001, 9: 59-65.
Dunyo SK, Appawu MA, Nkrumah FK, Baffoe-Wilmot A, Pedersen EM, Simonsen PE: Lymphatic filariasis on the coast of Ghana. Trans Roy Soc Trop Med Hyg. 1996, 90: 634-638. 10.1016/S0035-9203(96)90414-9.
Bryan JH, Mcmahon P, Barnes A: Factors affecting transmission of Wuchereria bancrofti by Anopheline mosquitoes. 3. Uptake and damage to ingested microfilariae by An. gambiae, An. arabiensis, An. merus and An. funestus in East Africa. Trans Roy Soc Trop Med Hyg. 1990, 84: 265-268. 10.1016/0035-9203(90)90281-I.
Bryan JH, Southgate BA: Factors affecting transmission of Wuchereria bancrofti by Anopheles mosquitoes. 1. Uptake of microfilariae. Trans Roy Soc Trop Med Hyg. 1988, 82: 128-137. 10.1016/0035-9203(88)90286-6.
McGreevy PB, Kolstrup N, Tao J, Mcgreevy MM, Marshall TF: Ingestion and development of Wuchereria bancrofti in Culex quinquefasciatus, Anopheles gambiae and Aedes aegypti after feeding on humans with varying densities of microfilariae in Tanzania. Trans Roy Soc Trop Med Hyg. 1982, 76: 288-296. 10.1016/0035-9203(82)90170-5.
Bryan JH, Di Deco MA, Petrarca V, Coluzzi M: Inversion polymorphism and incipient speciation in Anopheles gambiae s.s. in the Gambia, West Africa. Genetica. 1982, 59: 167-176. 10.1007/BF00056539.
Coluzzi M, Petrarca V, Di Deco MA: Chromosomal inversion intergradation and incipient speciation in Anopheles gambiae. Bollettino di Zoologia. 1985, 52: 45-63. 10.1080/11250008509440343.
Coluzzi M, Sabatini A, Petrarca V, Di Deco MA: Chromosomal differentiation and adaptation to human environments in the Anopheles gambiae complex. Trans Roy Soc Trop Med Hyg. 1979, 73: 483-497. 10.1016/0035-9203(79)90036-1.
Hunter JM: Elephantiasis: a disease of development in north east Ghana. Soc Sci Med. 1992, 35: 627-645. 10.1016/0277-9536(92)90001-7.
Carnevale P, Guillet P, Robert V, Doannio J, Coosemans M, Mouchet J, D F: Diversity of malaria in rice growing areas of the Afrotropical region. Parassitologia. 1999, 41: 273-276.
Coluzzi M: Advances in the study of Afro tropical malaria vectors. Parassitologia. 1993, 35: 23-29.
Powell JR, Petrarca V, DT A, Caccone A, Coluzzi M: Population structure, speciation and introgression in the Anopheles gambiae complex. Parassitologia. 1999, 41: 101-111.
Della Torre A, Fanello C, Akogbeto M, Dossou-yovo J, Favia G, Petrarca V, Coluzzi M: Molecular evidence of incipient speciation within Anopheles gambiae s.s. in West Africa. Insect Mol Biol. 2001, 10 (1): 9-18. 10.1046/j.1365-2583.2001.00235.x.
Michel AP, Guelbeogo WM, Grushko O, Schemerhorn BJ, Kern M, Willard MB, Sagnon N, Costantini C, Besansky NJ: Molecular differentiation between chromosomally defined incipient species of Anopheles funestus. Insect Mol Biol. 2005, 14 (4): 375-387. 10.1111/j.1365-2583.2005.00568.x.
Kamau L, Lehmann T, Hawley WA, Orago AS, Collins FH: Microgeographic genetic differentiation of Anopheles gambiae mosquitoes from Asembo Bay, western Kenya: a comparison with Kilifi in coastal Kenya. AmJTrop Med Hyg. 1998, 58: 64-69.
Lehmann T, Besansky NJ, Hawley WA, Fahey TG, Kamau L, Collins FH: Microgeographic structure of Anopheles gambiae in western Kenya based on mtDNA and microsatellite loci. Mol Ecol. 1997, 6: 243-253. 10.1046/j.1365-294X.1997.00177.x.
Favia G, Della TA, Bagayoko M, Lanfrancotti A, Sagnon N, Toure YT, Coluzzi M: Molecular identification of sympatric chromosomal forms of Anopheles gambiae and further evidence of their reproductive isolation. Insect Mol Biol. 1997, 6: 377-383. 10.1046/j.1365-2583.1997.00189.x.
Slotman MA, Tripet F, Cornel AJ, Meneses CR, Lee Y, Reimer LJ, Thiemann TC, Fondjo E, Fofana A, Traore SF: Evidence for subdivision within the M molecular form of Anopheles gambiae. Mol Ecol. 2007, 16 (3): 639-649.
Gentile G, Slotman M, Ketmaier V, Powell JR, Caccone A: Attempts to molecularly distinguish cryptic taxa in Anopheles gambiae s.s. Insect Mol Biol. 2001, 10: 25-32. 10.1046/j.1365-2583.2001.00237.x.
Awolola TS, Oduola AO, Oyewole IO, Obansa JB, Amajoh CN, Koekemoer LL, Coetzee M: Dynamics of knockdown pyrethroid insecticide resistance alleles in a field population of Anopheles gambiae s.s. in south-western Nigeria. J Vector Borne Dis. 2007, 44 (3): 181-188.
Diabate A, Baldet T, Chandre C, Dabire KR, Kengne P, Guiguemde TR, Simard F, Guillet P, Hemingway J, Hougard JM: KDR mutation, a genetic marker to assess events of introgression between the molecular M and S forms of Anopheles gambiae (Diptera: Culicidae) in the tropical savannah area of West Africa. J Med Entomol. 2003, 40 (2): 195-198. 10.1603/0022-2585-40.2.195.
Weill M, Chandre F, Brengues C, Manguin S, Akogbeto M, Pasteur N, Guillet P, Raymond M: The kdr mutation occurs in the Mopti form of Anopheles gambiae s.s. through introgression. Insect Mol Biol. 2000, 9 (5): 451-455. 10.1046/j.1365-2583.2000.00206.x.
African Network for Vector Resistance: Atlas of insecticide resistance in malaria vectors of the WHO African region. 2005, Harare: World Health Organization Regional Office for Africa
Corbel V, N’Guessan R, Brengues C, Chandre F, Djogbenou L, Martin T, Akogbéto M, Hougard J, Rowland M: Multiple insecticide resistance mechanisms in Anopheles gambiae and Culex quinquefasciatus from Benin, West Africa. Acta Trop. 2007, 101 (3): 207-216. 10.1016/j.actatropica.2007.01.005.
Ranson H, N’guessan R, Lines J, Moiroux N, Nkuni Z, Corbel V: Pyrethroid resistance in African anopheline mosquitoes: what are the implications for malaria control?. Trends Parasitol. 2011, 27 (2): 91-98. 10.1016/j.pt.2010.08.004.
Yewhalaw D, Wassie F, Steurbaut W, Spanoghe P, van Bortel W, Denis L, Tessema D, Getachew Y, Coosemans M, Duchateau L: Multiple Insecticide Resistance: An Impediment to Insecticide-Based Malaria Vector Control Program. PLoS One. 2011, 6 (1): e16066-10.1371/journal.pone.0016066.
McCarroll L, Paton MG, Karunaratne SHPP, Jayasuryia HTR, Kalpage KSP, Hemingway J: Insecticides and mosquito-borne disease. Nature. 2000, 407 (6807): 961-962. 10.1038/35039671.
Hemingway J, Ranson H: Insecticide Resistance in Insect Vectors of Human Disease. Ann Rev Entomol. 2000, 45 (1): 371-391. 10.1146/annurev.ento.45.1.371.
Kelly-Hope LA, Diggle PJ, Rowlingson BS, Gyapong JO, Kyelem D, Coleman M, Thomson MC, Obsomer V, Lindsay SW, Hemingway J: Negative spatial association between lymphatic filariasis and malaria in West Africa. Trop Med Int Health. 2006, 11 (2): 129-135. 10.1111/j.1365-3156.2005.01558.x.
Bayoh MN, Thomas CJ, Lindsay SW: Mapping distributions of chromosomal forms of Anopheles gambiae in West Africa using climate data. Med Vet Entomol. 2001, 15: 267-274. 10.1046/j.0269-283x.2001.00298.x.
de Souza D, Kelly-Hope L, Lawson B, Wilson M, Boakye D: Environmental Factors Associated with the Distribution of Anopheles gambiae s.s in Ghana; an Important Vector of Lymphatic Filariasis and Malaria. PLoS One. 2010, 5 (3): e9927-10.1371/journal.pone.0009927.
Sunish I, Rajendran R, Mani T, Munirathinam A, Dash A, Tyagi B: Vector control complements mass drug administration against bancroftian filariasis in Tirukoilur, India. Bull World Health Organ. 2007, 85 (2): 138-145. 10.2471/BLT.06.029389.
Ashton R, Kyabayinze D, Opio T, Auma A, Edwards T, Matwale G, Onapa A, Brooker S, Kolaczinski J: The impact of mass drug administration and long-lasting insecticidal net distribution on Wuchereria bancrofti infection in humans and mosquitoes: an observational study in northern Uganda. Parasit Vectors. 2011, 15 (4): 134-
Alilio M, Bygbjerg I, Breman J: Are Multilateral Malaria Research and Control Programs the Most Successful? Lessons from the Past 100 Years in Africa. AmJTrop Med Hyg. 2004, 71 (2): 268-278.
Stapleton D: Lessons of history? The anti-malaria strategies of the International Health Board and the Rockefeller Foundation from the 1920s to the era of DDT. Public Health Rep. 2004, 119: 206-215.
Kelly-Hope L, Ranson H, Hemingway J: Lessons from the past: managing insecticide resistance in malaria control and eradication programmes. Lancet Infect Dis. 2008, 8 (6): 387-389. 10.1016/S1473-3099(08)70045-8.
Lounibos LP, Conn JE: Malaria vector heterogeneity in South America. Am Entomol. 2000, 46: 238-249.
Gorgas W: Malaria prevention on the Isthmus of Panama. The Prevention of Malaria. Edited by: Ross R. 1910, New York: E. P. Dutton & Co, 346-352.
Sadasivaiah S, Tozan Y, Breman J: Dichlorodiphenyltrichloroethane (DDT) for indoor residual spraying in Africa: how can it be used for malaria control?. AmJTrop Med Hyg. 2007, 77 (6): 249-263.
Gyapong JO, Twum-Danso NAY: Global elimination of lymphatic filariasis: fact or fantasy?. Trop Med Int Health. 2006, 11: 125-128. 10.1111/j.1365-3156.2005.01542.x.
Schwab AE, Boakye DA, Kyelem D, Prichard RK: Detection of Benzimidazole resistance-associated mutations in the filarial nematode Wuchereria bancrofti and evidence for selection by Albendazole and Ivermectin combination treatment. AmJTrop Med Hyg. 2005, 73 (2): 234-238.
McCarthy J: Is anthelminthic resistance a threat to the program to eliminate lymphatic filariasis?. AmJTrop Med Hyg. 2005, 73: 232-233.
Pedersen EM, Mukoko DA: Impact of insecticide-treated materials on filaria transmission by the various species of vector mosquito in Africa. Ann Trop Med Parasitol. 2002, 96 (Suppl 2): S91-S95.
Zielke E, Chlebowsky HO: Studies on bancroftian filariasis in Liberia, West Africa V. The influence of treatment with Diethylcarbamazine and vector control on the transmission of Wuchereria bancrofti. Tropenmed Parasitol. 1980, 31: 444-458.
Boyd A, Won KY, McClintock SK, Donovan CV, Laney SJ, Williams SA, Pilotte N, Streit TG, de Rochars MVEB, Lammie PJ: A Community-Based Study of Factors Associated with Continuing Transmission of Lymphatic Filariasis in Leogane, Haiti. PLoS Negl Trop Dis. 2010, 4 (3): e640-10.1371/journal.pntd.0000640.
We declare that we have no conflicts of interest.
DKD prepared the initial draft of the manuscript, and all other authors added their contributions and comments. All authors read and approved the final version of the MS.
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de Souza, D.K., Koudou, B., Kelly-Hope, L.A. et al. Diversity and transmission competence in lymphatic filariasis vectors in West Africa, and the implications for accelerated elimination of Anopheles-transmitted filariasis. Parasites Vectors 5, 259 (2012). https://doi.org/10.1186/1756-3305-5-259
- Lymphatic Filariasis
- Anopheles vectors
- Vector-Parasite interactions
- West Africa