Mosquitoes genetically engineered to be resistant to Plasmodium parasites represent a promising novel approach in the fight against malaria. The insect immune system itself is a source of anti-parasitic genes potentially exploitable for transgenic designs. The Anopheles gambiae thioester containing protein 1 (TEP1) is a potent anti-parasitic protein. TEP1 is secreted and circulates in the mosquito hemolymph, where its activated cleaved form binds and eliminates malaria parasites. Here we investigated whether TEP1 can be used to create malaria resistant mosquitoes. Using a GFP reporter transgene, we determined that the fat body is the main site of TEP1 expression. We generated transgenic mosquitoes that express TEP1r, a potent refractory allele of TEP1, in the fat body and examined the activity of the transgenic protein in wild-type or TEP1 mutant genetic backgrounds. Transgenic TEP1r rescued loss-of-function mutations, but did not increase parasite resistance in the presence of a wild-type susceptible allele. Consistent with previous reports, TEP1 protein expressed from the transgene in the fat body was taken up by hemocytes upon a challenge with injected bacteria. Furthermore, although maturation of transgenic TEP1 into the cleaved form was impaired in one of the TEP1 mutant lines, it was still sufficient to reduce parasite numbers and induce parasite melanization. We also report here the first use of Transcription Activator Like Effectors (TALEs) in Anopheles gambiae to stimulate expression of endogenous TEP1. We found that artificial elevation of TEP1 expression remains moderate in vivo and that enhancement of endogenous TEP1 expression did not result in increased resistance to Plasmodium. Taken together, our results reveal the difficulty of artificially influencing TEP1-mediated Plasmodium resistance, and contribute to further our understanding of the molecular mechanisms underlying mosquito resistance to Plasmodium parasites.
We examined whether the natural anti-parasitic protein TEP1 can be harnessed to generate malaria resistant mosquitoes. We report the expression pattern of genes of the TEP1 immune pathway and the effects of both exogenous and enhanced endogenous expression of TEP1 on the development of Plasmodium in Anopheles gambiae. We found that exogenous expression of TEP1 increases resistance to Plasmodium in TEP1 mutants but not in a wild type background, and that enhancing expression of endogenous TEP1 does not increase resistance. We conclude that increased expression of TEP1 alone is not sufficient to render mosquitoes resistant to Plasmodium.
Citation: Volohonsky G, Hopp A-K, Saenger M, Soichot J, Scholze H, Boch J, et al. (2017) Transgenic Expression of the Anti-parasitic Factor TEP1 in the Malaria Mosquito Anopheles gambiae. PLoS Pathog 13(1): e1006113. doi:10.1371/journal.ppat.1006113
Editor: Kenneth D. Vernick, Institut Pasteur, FRANCE
Received: June 22, 2016; Accepted: December 6, 2016; Published: January 17, 2017
Copyright: © 2017 Volohonsky et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: All relevant data are within the paper and its Supporting Information files.
Funding: This work was funded by an Agence Nationale de la Recherche (ANR) young investigator grant to EM (project GEMM), by the European Commission FP7 projects INFRAVEC (grant agreement no. 228421), by an Investissements d'Avenir grant (ANR-11-EQPX-0022), by an ERC starting researcher grant to SAB (grant #260918), by the Institut National de la Santé et de la Recherche Médicale (INSERM U963), by the Centre National de la Recherche Scientifique (CNRS UPR9022), and by the University of Strasbourg. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Malaria is a devastating disease annually infecting over 200 million people worldwide, and is a leading cause of death in Sub-Saharan Africa . The malaria-causing Plasmodium parasites are vectored by Anopheline mosquitoes, which constitute the obligatory primary host for Plasmodium. Out of 462 described species of Anopheles mosquitoes, about 34 are dominant vectors of human malaria [2,3]. A. gambiae is the major vector of the most deadly parasite, P. falciparum, in Sub-Saharan Africa. Thanks to vector control and the availability of anti-malarial combination therapies, estimated global malaria cases and mortality rates between 2000 and 2015 have declined by 37% and 60%, respectively, falling to approximately 440,000 deaths annually. Despite this downward trend, the fight against malaria is complicated by the spread of genetic resistance to insecticides in mosquitoes, and to anti-malarial drugs in Plasmodium. To prevent a reversal in the current malaria decline, new vector control strategies need to be developed.
Vector control strategies based on genetically modified mosquitoes have been advocated for over 15 years to complement existing anti-malaria interventions (reviewed by  and ). Interventions based on the sterile insect technique (SIT) [6,7] or its transgenic variants, such as the Release of Insects carrying a Dominant Lethal (RIDL) technique deployed in recent years against the dengue vector mosquito Aedes aegypti [8,9,10], are unpractical on the vast geographical scales of malaria transmission. Gene drive-based strategies, whereby a desired genetic character (female sterility for population suppression, malaria resistance for population replacement) is inserted on a selfish genetic element designed to spread throughout a target population, have raised great interest [11,12,13] but their development has been limited by the paucity of molecular engineering tools. Today, these prospects are regaining momentum thanks to the advent of the CRISPR-Cas9 system, which provides a simple means to build a gene drive construct [14,15]. Major leaps towards establishing CRISPR-Cas9 gene drive designs for spreading malaria resistance and for population suppression have been accomplished in two recent studies [16,17], moving these approaches a step closer to implementation. However, the capacity to modify, or even eradicate, an entire insect species poses serious ethical and environmental questions. While regional population suppression or eradication appears desirable for invasive insect species such as Aedes aegypti that is not part of the native ecosystem in most of its current range, the importance of the role that a “legitimate” species like A. gambiae in Sub-Saharan Africa plays in its ecosystem needs to be examined. In this case, gene drive strategies aiming at population replacement with malaria-refractory mosquitoes rather than population suppression may be preferred, at least as a first test of gene drive interventions within a malaria eradication program. Therefore, candidate genes that would confer mosquito resistance against malaria parasites need to be screened and validated for efficiency in transgenic mosquitoes.
When Plasmodium ookinetes, the motile stage of the parasite that forms in the blood meal of female mosquitoes, traverse the mosquito midgut epithelium and reach the basal lamina facing the insect’s hemocoele, they are attacked by the mosquito’s innate immune system. This process has been mostly studied in A. gambiae mosquitoes in combination with the murine parasite P. berghei, which offers a convenient model to study Anopheles—Plasmodium interactions in the laboratory . The killing of ookinetes at the basal lamina is associated with direct binding of mosquito Thioester protein 1 (TEP1) to the ookinete surface . TEP1 is a homolog of the mammalian C3 complement factor. Like C3, which circulates in mammalian blood, TEP1 is a soluble hemolymph protein and its activity is dependent on an intact thioester bond thought to mediate covalent binding to bacteria and parasites [19,20]. TEP1 is secreted as a full-length protein (TEP1-full) and cleaved to produce activated TEP1 (TEP1-cut) in which the two cleaved parts of TEP1 remain connected by a disulfide bond [20,21,22]. TEP1-cut circulates in the hemolymph as a complex with two leucine rich repeat (LRR) proteins, LRIM1 and APL1C. Knocking down TEP1 itself or any of these LRR genes results in the disappearance of TEP1-cut from the hemolymph, and eliminates parasite killing [21,22]. However, TEP1 does not appear to directly lyse pathogens and the precise mechanism of killing remains unknown.
TEP1 has also been shown to act in mosquito resistance against the human parasite P. falciparum, though parasite virulence factors such as the ookinete surface protein Pfs47 have evolved in some parasite strains to counteract the TEP1-dependent immune response [23,24]. In addition, several TEP1 alleles are present in mosquito populations. The abundant TEP1*S alleles (hereinafter termed TEP1s) are associated with susceptibility to P. berghei infection, supporting the production of large numbers of oocysts. The less frequent TEP1*R1 allele (hereinafter TEP1r) confers high resistance to P. berghei, and leads to parasite melanization . Consistently, the laboratory L3-5 line that was selected based on the ability to kill P. cynomolgi  also kills all P. berghei parasites, is homozygous for TEP1r and exhibits high levels of parasite melanization. Furthermore, silencing TEP1 in mosquitoes before infection further increases parasite loads in susceptible mosquitoes and abolishes resistance and parasite melanization in refractory mosquitoes . Recently obtained TEP1 mutants exhibit the same phenotype .
Melanization is a powerful anti-parasitic and anti-microbial defense response used by insects to isolate and kill invading pathogens. The biochemical process has been well characterized in Drosophila and shown to be tightly regulated by both positive and negative effectors . Recognition of pathogens triggers activation of a serine protease cascade that culminates in the cleavage of the inactive circulating Prophenoloxidase (PPO) to its active Phenoloxidase (PO) form. PO then oxidizes quinones that polymerize to form melanin, which is in turn cross-linked with proteins and deposited on the pathogen. This chain reaction is localized in close proximity to the pathogen. High local levels of reactive oxygen species arising from quinone oxidation reactions also contribute to pathogen killing . In mosquitoes, this serine protease cascade is negatively regulated by serpins and activated by several CLIP domain proteases [30,31]. In resistant mosquitoes, silencing either TEP1, LRIM1 or APL1C abolishes melanization and allows parasite survival [19,21,22,32]. Furthermore, it is possible to disrupt melanization by knocking down genes that regulate actin polymerization without affecting the killing of parasites . These results suggest that the role of TEP1r in the resistant L3-5 mosquitoes is first in killing the parasites, then in promoting their melanization.
Here, we investigated the possibility of rendering mosquitoes resistant to P. berghei by transgenic expression of TEP1r. Together with insights regarding the potential of TEP1 transgenes as malaria control agents, our observations reveal new aspects of TEP1 biology, including expression pattern, promoter characterization, competition between TEP1 allelic forms, and anti-parasitic activity.
The TEP1, LRIM1 and APL1C expression pattern in transgenic reporter mosquitoes
In order to over-express TEP1 in mosquitoes in the endogenous source tissue, we first sought to determine which cells express TEP1 mRNA and attempted to perform RNA in situ hybridization in both larva and adult mosquitoes. However, the fat body tissue did not withstand the procedure and was lost from the analysis. Thus, we constructed a transgenic reporter line expressing GFP under control of the TEP1 promoter. For this, we cloned a 3.1 kb genomic DNA fragment located 5’ of the TEP1s gene from the A. gambiae G3 strain, ending at the TEP1s initiator ATG codon. Transfection assays in Drosophila S2 cells confirmed that this cloned TEP1s 5’ region is responsive to bacterial challenge (see below), as is the endogenous TEP1 gene . Investigation of the expression pattern of GFP in the transgenic mosquitoes revealed strong expression in the fat body tissue at larval (Fig 1a and 1b), pupal (Fig 1c and 1d) and adult stages (Figs 1n and 2). In addition, intense GFP expression was detected in cells of the midgut proventriculus (cardia) of adult mosquitoes, both males and females, regardless of blood feeding (Fig 1i and 1j, and S1a and S1b Fig). Other tissues showing some GFP expression included the oviduct, and more variably, the Malpighian tubules (S1c Fig). GFP was expressed in fat body loosely attached to the testis, but was not observed in the male reproductive organs themselves.
The 3xP3 promoter drives expression of transgenesis markers in eyes and nerve cells. a. Control 3xP3-RFP transgenic A. gambiae larva, image is a merge of green and red channels. Red arrows point to RFP expression in nerve cells, used as transgenesis marker (tm). b. TEP1-GFP, 3xP3-RFP larva. Arrows point to some of the lobes of the fat body expressing GFP. Note the fine architecture of thoracic fat body revealed by GFP expression. c. control wild type pupa, showing little auto fluorescence in the green channel. d. TEP1-GFP, 3xP3-RFP pupa showing GFP expression in fat body (fb, white arrows) and RFP expression in the eye (red arrows, tm). e-g. Larva carrying both ppo6-RFP, 3xP3-YFP and TEP1-GFP, 3xP3-RFP. RFP is expressed in hemocytes (white arrows) while GFP is expressed in fat body cells. YFP and RFP transgenic markers (red arrows, tm) are expressed in the nervous system. Scale bar = 200 μm h. RFP and YFP expression in ppo6-RFP, 3xP3-YFP pupa, showing RFP expression in hemocytes (hc). White arrows point to some RFP expressing hemocytes. Transgenesis YFP marker is expressed in the eye (red arrow, tm). i. Midgut of TEP1-GFP,3xP3-RFP female 24h after blood feeding, showing distinct GFP expression in proventriculus. (pv) j. Close-up on a proventriculus expressing GFP in TEP1-GFP gut. k. LRIM1-GFP,OpIE2-pac larva showing GFP expression in the fat body, alongside a control (wt) larva. l. Larva expressing APL1C-GFP, 3xP3-CFP showing GFP expression in the fat body (white arrows) and CFP transgenesis marker expression (red arrows, tm) in the nervous system (delineated with a thin line) m. APL1C-GFP,3xP3-CFP pupa expressing GFP in the fat body (white arrows) and CFP transgenesis marker in the eyes (tm, red arrow). n. TEP1-GFP (1) and APL1C-GFP (3) adult females with intense reporter expression in the fat body, visible through the cuticle, alongside a control female (2). Images a-h, j-m were acquired on a Zeiss Axiovert 200M microscope using a 5x or 10x objective. Images i and n were acquired on a Nikon SMZ18 binocular fluorescence microscope. Scale bar = 500μm except for d-h, l-m: 200 μm.
a. Dissected carcass of TEP1-GFP,3xP3-RFP and Lp-RFP, 3xP3-CFP mosquito exposing the fat body that shows GFP and RFP expression. Merged image shows co-expression of Lp and TEP1 reporters in the fat body. Scale bar = 200 μm. b-c. Stained carcasses of wild type (b) and mosquitoes treated with dsTEP1 (TEP1KD (c)) showing TEP1 antibody staining (green) in Lp-expressing fat body cells. Note reduction in TEP1 staining in TEP1KD carcasses. Dapi stained cell nuclei (blue). Shown are z-projections of confocal images, scale bar = 10μm. Images were collected on a Zeiss LSM 710 confocal microscope.
As a control for fat body and hemocyte expression we used the Lipophorin (Lp) promoter-driven RFP reporter line constitutively expressing RFP in the fat body and the hemocyte-specific PP06-RFP line . Comparing the expression of TEP1-GFP to the Lp-RFP pattern shows similar expression in the same cells in dissected carcass tissues (Fig 2a). Mosquitoes carrying both reporter genes showed perfect GFP/RFP overlap. Upon crossing TEP1-GFP mosquitoes to the hemocyte reporter PPO6-RFP line, the observed RFP-positive hemocytes were never positive for GFP, indicating that the TEP1 reporter is not strongly expressed in the hemocytes that express PPO6 (Fig 1e–1h). Although the reporter mosquitoes did not display obvious GFP-positive hemocytes, we do not rule out a possible expression of endogenous TEP1 in some hemocytes, as the cloned regulatory sequences may lack distant hemocyte-specific enhancers.
To identify the expression pattern of other genes known to act in the TEP1 pathway, we also constructed transgenic reporter lines expressing GFP under the control of the promoters of the leucine-rich proteins LRIM1 and APL1C that associate with TEP1 in the hemolymph. Both reporter lines showed a GFP expression pattern similar to TEP1, namely expression in the fat body at all developmental stages (Fig 1k–1n). However, neither LRIM1-GFP nor APL1C-GFP exhibited GFP expression in the proventriculus. Of note, all these reporters were created using the same docking line, and are thus subjected to the same potential positional effects. Many other fluorescent reporter constructs inserted at the same locus exhibit different, promoter-specific patterns of expression , indicating that the TEP1, LRIM1 and APL1C promoters must contain sequences determining fat body-specific expression.
In mosquitoes, fat body cells are challenging to manipulate. Dissection of mosquitoes in buffer results in immediate loss of large parts of the fat body. The fat body cells that remain attached to the carcass detach easily during fixation and disappear during permeabilization in buffers containing detergents. To verify the expression of TEP1 in the fat body cells that remain attached to dissected mosquito carcasses, we performed an antibody staining of fixed samples using a modified protocol (see materials and methods). Indeed, careful examination showed that some fat body cells that express the fat body specific protein Lipophorin (Lp) also stain positive for TEP1 (Fig 2b). In mosquitoes where TEP1 was silenced by RNAi, this fat body TEP1 staining was markedly reduced (Fig 2c), indicating that the signal is TEP1-specific.
TEP1-GFP reporter expression varies greatly among individual mosquitoes
Larvae and adults of the transgenic TEP1-GFP reporter line express GFP at strikingly variable levels (S1d and S1e Fig). We followed the levels of GFP during larval development (S2 Fig) and found an increase in GFP levels in time, most fourth instar larvae having reached a maximum level of GFP expression, though striking differences from larva to larva persist until pupation. Newly eclosed adult mosquitoes also exhibit variable levels of GFP expression (S1e Fig), probably reflecting a high variability in TEP1 expression that contrasts with the highly reproducible expression level of the Lp-RFP reporter. We hypothesized that the variability in GFP expression reflected TEP1 induction by immune pathways  upon encounter with various microorganisms, which may differ from larva to larva. We tested whether there is a correlation between the level of GFP in adult mosquitoes and intensity of P. berghei infection. Adult mosquitoes were scored for GFP expression prior to infectious blood feeding and grouped according to weak or strong reporter expression level. Mosquitoes were infected and oocysts were counted 7 days post infection. S1 Table summarizes the result of 5 independent experiments, showing no significant differences in oocysts loads between the high and low GFP expressing mosquitoes in 4 out of 5 experiments.
Transgenic expression of TEP1 in the fat body
Given the localization of GFP expression under control of the TEP1 promoter, we decided to express the TEP1 transgene in adult fat body tissue. To avoid unnaturally high TEP1 expression throughout development, we used the blood-meal inducible Vg promoter. Vg is induced at high levels after blood feeding  peaking 24h after blood meal, at the time when P. berghei ookinetes reach the basal lamina and encounter circulating TEP1. This experimental design aimed at achieving high levels of TEP1 simultaneously to Plasmodium infection.
Since the TEP1r allele is associated with refractoriness to P. berghei infection and shown to be more potent in Plasmodium killing, we based our construct on the TEP1r allele. TEP1r cDNA was cloned under the Vg promoter and injected into the TEP1s-containing X1 docking line , to create the Vg-TEP1r,3xP3-RFP transgenic line (henceforth referred to as Vg-TEP1r). Analysis of TEP1r mRNA in the transgenic mosquitoes (S3a Fig) showed blood meal induction of TEP1r similar to induction of Vg . Like Vg mRNA, TEP1r mRNA levels monitored with TEP1r-specific primers peaked 24h after blood meal and dropped gradually in the following days. However, Western blot analysis of the transgenically expressed TEP1r protein in the TEP1s background did not reveal a notable increase in TEP1 protein levels in the transgenic mosquitoes 24h after blood feeding (S3b Fig), suggesting tight post-transcriptional control of hemolymph TEP1 protein levels.
In order to verify expression from the Vg-TEP1r transgene, we introduced it into two different TEP1 null mutant lines . The TEP1Δct2 mutant has a nonsense mutation causing a premature stop codon and loss of the entire C-terminus. The TEP1ΔT mutant has a deletion of a threonine located 16 amino acids before the thioester cysteine. Both mutants lack detectable TEP1 protein in the hemolymph at 24h after blood feeding, but low levels of mutated TEP1 become detectable in old TEP1ΔT mosquitoes only. Samples from TEP1Δct2; Vg-TEP1r mosquitoes analyzed by polyclonal anti TEP1 antibodies showed the presence of both forms of TEP1, namely TEP1-full and TEP1-cut in the hemolymph expressed from the transgene (Fig 3a). In contrast, hemolymph samples from TEP1ΔT; Vg-TEP1r showed only the TEP1-full form (Fig 3b), suggesting that traces of the mutant TEP1ΔT protein inhibit maturation of wild-type TEP1 expressed from the transgene. In addition, TEP1ΔT (but not TEP1Δct2) mosquitoes show reduced levels of LRIM1 and APL1C (Fig 3a–3c and 3e). Unlike LRIM1 and APL1C depletion by RNAi silencing , this decrease does not result in massive TEP1-cut deposition on tissue (Fig 3d). Thus, traces of the mutant TEP1ΔT protein appear to downregulate both the endogenous LRIM1/APL1C complex and the cleavage of transgenic TEP1-full.
a. Western blot analysis of hemolymph from Plasmodium infected wild type (TEP1s), mutant (TEP1Δct2) and mutant mosquitoes ectopically expressing TEP1r (TEP1Δct2;TEP1r;) showing full (TEP1-full) and cleaved (TEP1-cut) TEP1 forms, LRIM1 and APL1C protein, 25 and 48h after infectious blood feeding. PPO2 is used as a loading control b. Western blot analysis of hemolymph from Plasmodium infected mosquitoes of the TEP1ΔT mutant background (TEP1ΔT), ectopically expressing TEP1r (TEP1ΔT; TEP1r) and wild type L3-5 mosquitoes expressing only the endogenous TEP1r allele (TEP1r). 3–4 day old mosquitoes were blood fed to induce the Vg promoter. Samples were collected 24h after blood meal. The membrane was probed with the indicated antibodies, including anti-Vg to confirm proper induction of the Vg promoter. Two independent samples were loaded for each condition to account for variability. c. Western blot analysis of hemolymph from control and TEP1 mutant mosquitoes showing the levels of APL1C and LRIM1. PPO2 is used as a loading control. Note the specific reduction of the two LRR proteins only in TEP1ΔT mosquitoes in which TEP1 lacks a single threonin. TEP1Δct1 and TEP1Δct2 are two different mutants lacking the entire C-terminus . d. Western blot analysis of carcasses from mosquitoes 48h after blood feeding showing the levels of TEP1-full and -cut in the indicated genotypes. Two independent samples of each genotype are shown to represent variability. Actin (upper band of the doublet) used as loading control. e. Western blot analysis of hemolymph from mosquitoes injected with heat-killed E. coli 24h after blood feeding comparing TEP1 levels in injected and non-injected mosquitoes of the indicated genotypes. Note the absence of transgenic TEP1r cleavage and reduced LRIM1 in the TEP1ΔT mutation background regardless of bacterial injection. PPO2 was used as a loading control.
It has been previously demonstrated that injection of bacteria into mosquitoes promotes TEP1 maturation and activates TEP1 transcription . Furthermore, shortly after bacteria injection, TEP1-cut binds to bacterial surfaces and acts as a convertase to recruit the full-length protein [38,39]. The recruited TEP1-full is then cleaved close to bacterial surfaces and increases bacterial opsonization, thus marking bacteria for phagocytosis by hemocytes . We tested whether injection of bacteria induced formation of the TEP1-cut form in the TEP1ΔT;Vg-TEP1r mosquitoes (Fig 3e). While the positive control TEP1r mosquitoes showed an increase in both TEP1-full and TEP1-cut after bacterial injection, transgenic TEP1-full in the TEP1ΔT;Vg-TEP1r mosquitoes’ hemolymph still failed to be converted to TEP1-cut.
Infection of TEP1r transgenic mosquitoes with P. berghei
In order to verify that the TEP1r transgene was functional, we infected TEP1 mutant mosquitoes complemented with the Vg-TEP1r transgene. The TEP1Δct2;Vg-TEP1r mosquitoes resemble the L3-5 line in that they express only the TEP1r allele. However, an important difference from the L3-5 line is that TEP1r is expressed exclusively in the fat body and only after a blood meal. In the TEP1ΔT;Vg-TEP1r line, only the full form of TEP1 is detectable in the hemolymph, which offers an opportunity to examine the activity of the TEP1-full form in the absence of detectable TEP1-cut.
P. berghei infection of TEP1Δct2;Vg-TEP1r was strikingly reduced compared to mutant controls, with some live oocysts and mostly melanized parasites (Fig 4a), indicating that the introduced TEP1r is fully functional and sufficient to kill parasites. Infection prevalence (S2 Table) in the transgenic is also significantly lower than in control Vg-GFP mosquitoes that express TEP1s only. P. berghei infection of TEP1ΔT;Vg-TEP1r, in which only the full form of TEP1 is detected, also resulted in a significant reduction in live oocyst numbers and in the concomitant appearance of high numbers of melanized parasites in some midguts compared to the non-rescued mutant (Fig 4b). High levels of melanization are reminiscent of the L3-5 infection phenotype, where complete refractoriness is achieved by TEP1r-mediated parasite killing followed by parasite melanization [19,33]. However, contrary to L3-5 that are completely refractory to the parasite, the rescued mutant lines which derive from the susceptible G3 background are not fully refractory to P. berghei infection, with about 70% of infected midguts containing live oocysts 7 days after infection (S2 Table) and infection intensities comparable to wild-type control G3 mosquitoes. In fact, expression of TEP1r in mutant backgrounds rescued the mutant at least to the level of the wild-type TEP1s-carrying G3 line in terms of prevalence and intensity, and further conferred a gain-of-function phenotype (melanization) (Fig 4a). In the TEP1ΔT;Vg-TEP1r line, it is striking that transgenic TEP1r appears to be functional in spite of its impaired maturation into the TEP1-cut form. These results imply either that TEP1 cleavage may be dispensable for some of its functions, or that low levels of TEP1-cut that we could not detect in the hemolymph (Fig 3b and 3e) or on parasites (Fig 5) may be sufficient for function. The formation of TEP1-cut at foreign surfaces is dependent on a convertase complex controlled by SPCLIP1 . To test if maturation of TEP1-full into TEP1-cut is required for the observed phenotype, we silenced SPCLIP1 by dsRNA injection in TEP1ΔT;Vg-TEP1r mosquitoes (S1 File). This fully abolished melanization and tended to increase parasite numbers, suggesting that some TEP1r cleavage by the convertase complex, though undetectable, must be required for activity of the TEP1r transgene.
a. P. berghei infection of TEP1Δct2 mutant mosquitoes rescued with transgenic TEP1r. Shown are the number of live parasites (green circles) and melanized parasites (black circles) in the midguts of mosquitoes 7 days after infection. Control mosquitoes are TEP1 mutant alone (TEP1Δct2) and transgenic mosquitoes expressing GFP instead of TEP1r (Vg-GFP). b. P. berghei infection of TEP1ΔT mutant mosquitoes compared to TEP1ΔT rescued with transgenic TEP1r (TEP1ΔT;Vg-TEP1r). c. P. berghei infection of transgenic mosquitoes expressing TEP1r in a wild type TEP1s background. Live (green circles) and melanized (black circles) parasites are compared in wild type (TEP1s) and transgenic (TEP1s;Vg-TEP1r) mosquitoes. d. P. berghei infection of transgenic TEP1r mosquitoes in wild type TEP1s background after TEP1 allele-specific knockdown. Compared are transgenic mosquitoes treated with dsLacZ, dsTEP1s and dsTEP1r, 3 days prior to infection. For all P. berghei infections, experiments were performed at least 3 times, representative experiments are shown. The raw numbers of parasites and calculated p values for all infections are provided in S2 Table.
TEP1 antibody staining (red) of dissected midguts 24 h after infection with GFP-expressing P. berghei. Shown are wild type mosquitoes expressing the TEP1s allele (TEP1s), wild type L3-5 mosquitoes expressing the TEP1r allele (TEP1r), mosquitoes transgenically expressing TEP1r in a wild type TEP1s background (TEP1s;Vg-TEP1r), mutant TEP1 mosquitoes (TEP1ΔT), and mutant mosquitoes transgenically expressing TEP1r (TEP1ΔT;Vg-TEP1r). Ookinetes express GFP (green) and nuclei are stained with Dapi (blue). Images are stacks of confocal z-sections, scale bar = 20 μm
Importantly, transgenic expression of TEP1r exclusively in the fat body using the Vg promoter rescued the TEP1 loss-of-function mutations (Fig 4a and 4b), showing that TEP1 produced in the fat body and secreted into the hemolymph is sufficient for parasite killing.
We tested whether expressing TEP1r in a wild type background where TEP1s is present could also reduce parasite loads after P. berghei infection. Oocyst counts revealed no difference in live oocyst numbers between the parental TEP1s line and the TEP1s;Vg-TEP1r transgenic line (Fig 4c, left panel). However, the number of melanized parasites was significantly elevated in these mosquitoes (Fig 4c, right panel). We verified that the increase in melanized parasites was attributable to the TEP1r transgene using allele specific RNAi. When transgenic TEP1r, but not endogenous TEP1s, was knocked down in the TEP1s;Vg-TEP1r transgenic line, the number of melanized parasites reverted to a level similar to control dsLacZ-injected mosquitoes (Fig 4d).
In the TEP1s;Vg-TEP1r line, transgenic TEP1r is induced to a peak level about 24 hours after a blood meal, possibly too late to efficiently fight parasite invasion. To induce TEP1 expression prior to the infectious blood meal and attempt to increase TEP1 concentration in the hemolymph, we offered a non-infectious blood meal and infected mosquitoes three days later, before the Vg promoter had returned to its off state. The results of such an experiment (S4 Fig) show no difference in infection levels between mosquitoes that were pre-induced by blood meal and naïve mosquitoes.
Binding of TEP1 to parasites
We verified that transgenic TEP1r binds to parasites in the TEP1Δct2;Vg-TEP1r line (S5 Fig) and asked whether this was also the case in TEP1ΔT;Vg-TEP1r mosquitoes in which formation of the mature TEP1-cut form is inhibited. To this end, we performed immuno-histochemical staining of TEP1ΔT;Vg-TEP1r midguts 24h after infection using TEP1 specific antibodies (Fig 5). Results show that in the presence of TEP1ΔT, transgenic TEP1r protein is not detectable on ookinete surfaces, despite its observed, SPCLIP1 dependent, anti-parasitic and melanization activity.
We tested whether the fat body-expressed, full length TEP1r in the TEP1ΔT;Vg-TEP1r line can enter hemocytes after bacterial injection. To this end we examined TEP1 staining in carcasses of blood fed mosquitoes, injected with heat killed E. coli, 24h after blood meal (Fig 6). Results show that in blood-fed TEP1ΔT;Vg-TEP1r mosquitoes, TEP1r artificially induced in the fat body by the blood meal accumulated in the hemocytes only when mosquitoes were injected with E. coli. Control wild type mosquitoes showed that TEP1 accumulation in hemocytes depended on bacterial injection, regardless of blood feeding. The TEP1ΔT mutant line, used here to control for the specificity of antibodies for TEP1, showed no TEP1 staining in hemocytes under any condition. These results show that TEP1 detection in hemocytes can result from uptake of what is most likely TEP1-labeled bacteria.
TEP1 antibody staining (red) of dissected mosquito carcasses after injection of heat killed E.coli. Nuclei are stained with Dapi (blue). Shown are wild type (TEP1s), TEP1s mutant (TEP1ΔT) and mutants complemented with transgenic TEP1r under control of the Vg promoter (TEP1ΔT;Vg-TEP1r). Compared are blood fed non injected (+BF), non blood fed injected (+E. coli) and blood fed, E. coli injected mosquitoes (+BF+ E. coli). scale bar = 20 μm.
Optimization of synthetic transcription factors to over-express endogenous TEP1
Since transgenic expression of TEP1r in a wild-type TEP1s background failed to produce refractory mosquitoes, we asked whether artificially elevating the levels of the endogenous TEP1s allele may lead to increased immunity against Plasmodium. To this aim, we stimulated expression of the endogenous TEP1 gene using synthetic transcription factors designed to bind specific promoter sequences.
Transcription Activator Like Effectors (TALEs) are transcription-activating proteins derived from Xanthomonas bacteria, containing a DNA-binding domain composed of nucleotide-binding repeats that can be arranged in the desired order to bind chosen DNA sequences [41,42,43]. In order to trigger over-expression of the endogenous TEP1 gene, we designed TALE proteins that bind specific DNA sequences in the promoter region of TEP1. To find the best potential binding position for a TALE, we first analyzed the 3 kb promoter region of TEP1 (S6 Fig). Using a luciferase reporter assay in Drosophila S2 cells and nested promoter deletions, we found that a 250 bp fragment of the promoter was sufficient to induce reporter activity. The minimal promoter sequence, harboring a potential NF-κB binding site, responded to the addition of bacteria to the culture medium by increased luciferase activity (S7 Fig). Mutating this NF-κB binding site abolished the reporter response to bacterial challenge (S8 Fig). This suggests that the NF-κB pathway of S2 cells can activate the mosquito TEP1 promoter, in agreement with the known activation of native TEP1 transcription by the mosquito NF-κB pathway . We used this minimal promoter to test several transcriptional activation domains for reporter activation by TALEs, namely those of yeast Gal4, Drosophila Heat Shock Factor 1 and Herpes virus VP16, and found that the VP16 activation domain fused to a TALE DNA-binding domain leads to highest reporter induction (S9 Fig). The VP16 domain was thus chosen as the activation domain for all further designed TALEs. TALEs without an activation domain did not increase TEP1 expression and served as negative controls.
We constructed five TALEs that bind at different positions along the TEP1 minimal promoter sequence (Fig 7a and S6 Fig) and tested their effect on reporter transcription in S2 cells (Fig 7b). Results show that TAL3 binding the closest to the transcription start site had no effect on reporter activity, while the other TALEs had a modest effect, increasing activity by about 1.5–2 fold. However, TAL6, binding the furthest from the transcriptional start site and just upstream of a sequence resembling a TATA box, triggered a strong, 20 fold increase in reporter activity. TAL6 was thus chosen to create transgenic mosquitoes with the aim of over-expressing endogenous TEP1.
a. Schematic representation of the ~3Kb TEP1 promoter (not to scale). Shown are potential NF-κB sites (GGGRNNYYCC) (light grey boxes) and potential TATA boxes (dark grey boxes). The minimal promoter (MP) shown to be active in cells is indicated by a black line. Numbers on the promoter indicate the distance from the ATG. White boxes represent the binding position of each designed TALE. b. Luciferase assay in S2 cells showing the effect of TALEs on the minimal TEP1 promoter. Different TALE constructs all carrying a VP16 activation domain and placed under the Drosophila actin5c promoter were co-transfected into S2 cells together with a firefly luciferase reporter gene under control of the minimal TEP1 promoter. A plasmid carrying GFP placed under the same promoter as TALEs was used as reference for basal promoter activity. The TEP1 promoter was further induced by addition of heat killed E. coli to the cells. Luciferase activity was normalized to the basal promoter activity without TALEs. c. qRT-PCR to assess the level of TALE and TEP1 mRNA in transgenic mosquitoes expressing Vg-TAL6 comparing functional TALE with VP16 activation domain (Vg-TAL6vp16) and control line expressing the same TALE without activation domain (Vg-TAL6ΔAD), with or without induction of the Vg promoter by a blood meal 24h prior to mRNA extraction. d. qRT-PCR of transgenic mosquitoes constitutively expressing Lp-TAL6 or Lp-TAL0 or both, showing the level of TEP1 mRNA. Levels of mRNA in each sample are normalized to wt and to the housekeeping reference gene RPL19. e Western blot analysis of transgenic mosquitoes constitutively expressing Lp-TAL6 or Lp-TAL0 or both. Wild type mosquitoes are used as controls. Shown are the bands for the full length and the cleaved forms of TEP1 as well as PPO2 as loading control. 2 samples for each mosquito line are presented to show sample variation. f. Quantification by densitometry of the TEP1 bands in (e). g. P. berghei infection of Vg-TALvp16 transgenic mosquitoes. h. P. berghei Infection of transgenic mosquitoes constitutively expressing TAL0, TAL6 or both under the Lp promoter. In all infections, the empty docking line (wtX1) serves as control. Live oocysts (green circles) in each midgut are counted 7 days after infection. Number of oocysts and infection data are in S3 Table.
In plants, natural and artificial TALEs induce target gene expression from alternative, TALE-specific transcription start sites [44,45]. We investigated whether TALEs triggered TEP1 expression through an alternative transcription site when transfected with the luciferase reporter in S2 cells. PCR products from the 5' RACE assay were sequenced and revealed that unlike in plants, both TAL0 and TAL6 preserved the normal transcriptional start site of the mRNA which remained located 43 bp upstream of the ATG (S6 Fig).
Transgenic mosquitoes expressing TALEs to drive endogenous TEP1 expression
We generated several transgenic lines that express TALEs designed to bind and activate the TEP1 promoter. Our first choice of promoter for the expression of the synthetic transcription factor itself was the inducible fat body specific Vg promoter, in order to increase endogenous TEP1 levels after a blood meal, concomitant with Plasmodium parasite invasion. TAL6 fused to a VP16 (TAL6vp16) activation domain was chosen due to its high activity in S2 cells. A control transgenic line was created with the same TAL6 lacking an activation domain (TAL6ΔAD). Analysis of mRNA after blood feeding revealed that in both transgenic lines TALEs are induced by a blood meal, more efficiently in the case of Vg-TAL6vp16 (Fig 7c). Furthermore, TAL6vp16, but not TAL6ΔAD, induced a two-fold elevation in TEP1 mRNA levels. This elevation in the endogenous levels of TEP1 mRNA is modest compared to the 20-fold average elevation of the reporter in the cell line.
Since the Vg promoter triggers a pulse of transcription after a blood meal, TALEs may activate TEP1 too transiently to achieve a significant effect. Therefore, we also tested if a constitutive fat-body promoter would durably induce high levels of endogenous TEP1. For this, TAL6vp16 and TAL0vp16 were placed under the control of the Lp promoter, constitutively expressed in the fat body in larvae, pupae and adults. We included TAL0vp16 in addition to TAL6vp16 despite its modest effect in S2 cells (~1.5 fold increase, Fig 7b) because of its unique binding position on the NF-κB binding site. TAL0vp16 was designed to bind and activate not only the promoter of TEP1, but also similar sequences found in the promoters of APL1C and LRIM1, two proteins that are known to bind TEP1 and contribute to its activity (See Methods).
Analysis of TEP1 mRNA in transgenic mosquitoes that constitutively express TAL6vp16 and/or TAL0vp16 (Fig 7d) revealed a maximum of 2-fold induction of endogenous TEP1 mRNA in mosquitoes that expressed both TALES simultaneously (progeny of a cross between the two lines). Western blot analysis of TEP1 in these mosquitoes (Fig 7e) confirmed a 3–4 fold increase in TEP1 protein levels circulating in the hemolymph (Fig 7f). We thus proceeded to test whether this elevation in TEP1 levels in the hemolymph had any effect on parasite loads after Plasmodium infection.
Infection of the blood meal inducible Vg-TAL6vp16 transgenic line did not result in any significant change in parasite loads (Fig 7g). Likewise, analysis of parasite loads after infection of the constitutively expressing Lp-TAL6vp16 and Lp-TAL0vp16 lines did not show any significant difference in oocyst numbers between transgenic and control lines (Fig 7h).
TEP1 pathway genes are expressed mainly in the fat body
TEP1 is a secreted protein that circulates in the hemolymph of mosquitoes at all developmental stages starting from larval stages . Previous observations suggested that TEP1 is produced by hemocytes and secreted from these cells as a full-length protein which is then cleaved in the hemolymph . Evidence to support this model included immuno-histochemical staining of mosquito tissues that showed TEP1 accumulation inside hemocytes, particularly after bacterial challenge and 24-48h after infection with P. berghei [22,35,46]. However, these results may also be explained by uptake of TEP1 protein, or TEP1-labeled particles, by hemocytes. In addition, analysis of RNA expressed by hemocytes using microarrays has shown that TEP1 transcript is present in these cells, but not enriched compared to whole female tissues, and is not further induced by infection . TEP1 did not emerge as a hemocyte transcript in the hemocyte transcriptomics study of Pinto et al. . Of note, it is technically challenging to acquire a pure population of hemocytes without contamination by fat body cells that detach into the hemolymph during sample collection . Here we obtain evidence that TEP1, LRIM1 and APL1C are expressed primarily in the fat body. This is similar to the expression pattern of many insect anti-microbial peptides [50,51] and to that of some Drosophila TEP family member genes as determined by in situ hybridization . In mammals, complement proteins phylogenetically and functionally homologous to TEP1 are expressed and secreted from the liver (,reviewed in ). Interestingly, some of the functions of the liver are performed by the fat body in insects.
We crossed the TEP1-GFP reporter mosquitoes to our hemocyte-specific PPO6-RFP line, and observed that the DsRed-positive hemocytes were GFP negative. We note that this result does not rule out that sub-populations of hemocytes not expressing the PPO6 promoter may also express TEP1; fine transcriptomic analyses will be required to quantitatively determine the contribution of each tissue to the global pool of circulating TEP1.
Our transgenic reporter lines also reveal that TEP1, but not APL1 and LRIM1, is also expressed in the proventriculus of adult mosquitoes. Interestingly, the proventriculus was found to be a site of immune gene expression in A. gambiae  and in other insects such as tsetse flies . In A. gambiae, mRNA transcripts of antimicrobial peptides Defensin 1, Cecropins, Gambicin, as well as TEP1, are enriched in the proventriculus . TEP1 is also expressed in the neighboring gastric caeca during larval stages . Future studies may clarify whether proventriculus-expressed TEP1 has a function that bypasses the requirement for LRM1 and APL1-C, perhaps in the lumen of the digestive tract where TEP1 could interact with the gut microbiota.
TEP1-GFP reporter expression does not reflect immune status
Variation in GFP levels among individual mosquitoes led us to test whether GFP fluorescence intensity correlates with infection outcome. We found no such correlation and concluded that GFP expression either did not reflect TEP1 levels in the mosquitoes at the time of P. berghei infection, or that TEP1 level variations do not correlate with resistance to the parasite. The lack of correlation between GFP levels and immune status may be due to the remarkable stability of GFP protein, which persists throughout mosquito life in the fat body after a blood feeding-induced pulse of expression in the Vg-GFP line  compared to the highly dynamic turnover of TEP1 protein, which disappears by 24h after RNAi silencing .
Transgenic expression of TEP1 in the fat body
Lysis of ookinetes at the basal lamina is associated with binding of TEP1 directly to the ookinete surface . However, TEP1 does not induce direct lysis of bound pathogens, and the molecular mechanism of killing remains unknown. It has been previously shown that TEP1-cut is the major form that binds ookinetes [21,22]. Binding of circulating TEP1-cut to pathogen surface triggers the recruitment of a convertase complex that requires the serine protease homologue SPCLIP1 and that cleaves circulating TEP1-full leading to further accumulation of TEP1-cut at the pathogen surface [38,39]. We expressed the TEP1r allele in two different TEP1 mutant backgrounds: TEP1ΔT carries a single threonine deletion that appears to destabilize the protein, as mutant TEP1ΔT protein becomes faintly detectable only in aged mosquitoes . TEP1Δct2 lacks the C-terminal third of the protein and is likely to be a complete null. In these two mutant backgrounds, transgenic TEP1r produced in the fat body and secreted into the hemolymph was sufficient to rescue parasite killing, and to trigger parasite melanization. Interestingly, in the TEP1ΔT background, but not in the TEP1Δct2 background, maturation of transgenic TEP1r-full to TEP1-cut appeared to be inhibited as we never detected circulating TEP1-cut in the hemolymph, even after bacterial injection. This suggests that very low amounts of the non-functional TEP1ΔT protein inhibit maturation of TEP1-full, perhaps by blocking the enzyme responsible for TEP1 cleavage in the hemolymph. Possibly related to this, LRIM1/APL1C levels are reduced in the TEP1ΔT, but not in the TEP1Δct2 mutant. In the TEP1ΔT;VgTEP1r mosquitoes, TEP1 binding is not detectable by antibody staining on ookinete surfaces, consistent with the lack of detectable circulating TEP1-cut form. Yet, both mutants rescued with TEP1r showed an increase in parasite melanization. We initially hypothesized that contrary to current views, processing of TEP1-full to TEP1-cut by the SPCLIP1-dependent convertase and accumulation of TEP1-cut at the parasite surface may be dispensable for parasite melanization in some contexts. However, disabling the TEP1 convertase complex through silencing SPCLIP1 in TEP1ΔT;VgTEP1r mosquitoes abolishes melanization and, to some extent, increases parasite numbers. Therefore, conversion of TEP1-full to TEP1-cut seems to be a prerequisite for parasite killing and melanization even in TEP1ΔT;VgTEP1r mosquitoes, but a large accumulation of TEP1-cut at the surface of parasites may not be necessary to trigger killing and melanization.
Another function of TEP1 in the hemolymph is the opsonization of bacteria [20,39,58,59], marking them for phagocytosis by hemocytes. Shortly after the injection of bacteria, TEP1 protein can be detected inside the hemocytes that are attached to dissected mosquito carcasses. The appearance of TEP1 inside these cells may be due to induced expression of TEP1 within hemocytes, presumably aimed at replenishing TEP1 levels in the hemolymph, or due to phagocytosis of TEP1-covered bacteria by hemocytes. We observed that in a TEP1 null mutant background, TEP1r expressed from a transgene in the fat-body could enter hemocytes. Our results suggest that TEP1 detected in hemocytes after bacterial challenge comes at least in part from uptake of circulating TEP1 protein.
TEP1r could be a candidate gene for creating malaria resistant mosquitoes by driving the gene into the wild mosquito population, for example using CRISPR-Cas9 gene drive [14,15]. This should not be achieved by replacement of endogenous TEP1s alleles with the more active TEP1r, as a few failed gene conversion events could result in Cas9-induced TEP1s loss-of-function mutations that would generate hyper-susceptible mosquitoes. Instead, the anti-parasitic factor should be driven into an independent neutral genomic locus. We thus tested whether over-expression of TEP1r in wild type background affects infection outcome. We found that transgenic TEP1r is indeed expressed in the presence of endogenous TEP1s, but fails to enhance parasite killing, while still able to stimulate melanization. Using allele specific knock-down we showed that the allelic difference between TEP1r and TEP1s is sufficient to explain the different intensities of the melanization reaction. In addition, silencing endogenous TEP1s in the same mosquitoes restored the ability of transgenic TEP1r to kill parasites and further elevated melanization (Fig 4d), as observed when transgenic TEP1r was expressed in a mutant background. This indicates that although less efficient than TEP1r for parasite killing, endogenous TEP1s protein is able to outcompete transgenic TEP1r for the parasite killing function. This is reminiscent of the apparent recessivity of TEP1r in TEP1s x TEP1r genetic crosses . Therefore, simple transgenic expression of TEP1r in a wild type background where TEP1s is the most frequent allele would not be sufficient to render a mosquito population refractory to Plasmodium infection.
Over-expressing endogenous TEP1
Since transgenic expression of TEP1r in a wild-type TEP1s background failed to produce refractory mosquitoes, we asked whether artificially elevating the levels of the endogenous TEP1s allele may lead to increased immunity against Plasmodium. To this aim, we stimulated expression of the endogenous TEP1 gene using synthetic transcription factors designed to bind specific sites in the TEP1 promoter.
We designed a luciferase reporter for TEP1 promoter activity and tested it in Drosophila S2 cells. The promoter contained an NF-κB binding site, which mediated elevation of reporter activity when S2 cells were treated with heat-killed bacteria. Thus, the cloned TEP1 promoter fragment is activated by the S2 cell NF-κB pathway, consistent with TEP1 activation by the mosquito NF-κB pathway .
Once we determined the optimal TALE sequence for binding TEP1 promoter, we created several transgenic mosquitoes lines that expressed TALEs either under an inducible promoter (Vg) or a constitutive fat body promoter (Lp). In all cases, the increase in endogenous TEP1 expression was very modest both at mRNA and protein levels, indicating that cell culture assays are poor predictors of TALE activity in vivo. TEP1 mRNA levels may be tightly regulated in vivo, or may depend on regulatory features that were absent or inactive in the S2 cells assays.
In wild type mosquitoes, some parasites are bound by TEP1 and killed, while others evade TEP1 binding. If the quantity of circulating TEP1 were the rate-limiting factor in parasite binding, we expected that even a modest 2-fold increase in TEP1 expression would yield increased resistance to Plasmodium. However, infection assays with mosquitoes that expressed TALEs and showed a 2 to 3-fold elevation in TEP1 levels did not show any increase in resistance. This is similar to the lack of increased parasite killing in mosquitoes expressing transgenic TEP1r in addition to endogenous TEP1s, and suggests that the survival of some parasites is not due to a lack of TEP1. The absence of effect of the TALE-mediated over-expression of TEP1s contrasts with the elevated melanization obtained by transgenic expression of TEP1r in mosquitoes carrying endogenous TEP1s, again confirming that enhancing melanization is an allelic property of TEP1r.
To conclude, our results indicate that simply augmenting the level of a given anti-parasitic factor may not be sufficient to achieve greater resistance levels, and biotechnological approaches aiming at rendering the mosquitoes resistant to malaria will need to integrate the full complexity of molecular interactions between immune factors.
Mosquito rearing and P. berghei infection
A. gambiae mosquitoes were maintained in standard conditions (28°C, 75–80% humidity, 12-hr/12-hr light/dark cycle). Larvae were raised in deionized water and fed finely ground TetraMin fish food. Adults were fed on 10% sucrose ad libitum and females were blood-fed on anaesthetized mice. For infection, mosquitoes were fed on CD1 mice infected with the P. berghei GFP-con 259cl2 clone (ANKA strain) that constitutively expresses GFP . Mice infected with Plasmodium berghei were sacrificed before they developed malaria symptoms by cervical dislocation. Mice used to blood feed and infect mosquitoes were anesthetized with a mix of xylazine and ketamine. Infected mosquitoes were maintained at 21°C, unfed mosquitoes were removed 24h post feeding. Seven days after infection, live midguts were mounted on microscope slides in PBS, photographed under fluorescent light, and parasites were counted on the pictures. Statistical significance of differences in parasite counts was evaluated with a Mann-Whitney non-parametric test.
Transgenic mosquitoes were created in the A. gambiae X1 attP docking line using the pDSA R/T/G/Y/P and pattB-RfB2 transgenesis vectors as described . The following plasmids were constructed by Goldengate cloning to generate transgenic mosquitoes: pDSAP-LRIM1-GFP, pDSAT-APL1-GFP. In the case of the TEP1-GFP,3xP3-RFP reporter and of the Vg-TEP1r,3xP3-YFP constructs, plasmids were assembled using Gateway cloning into pattB-RfB2 . Vg-TALE and Lp-TALE constructs were assembled by Goldengate cloning in pDSAR, pDSAT or pDSAG as described for TALEs . Plasmid sequences, as well as promoter and TALE modules are provided in supplementary file S1 Text. In the case of TAL0, we exploited the TAL repeat “NS” di-residue binding ambiguous bases to allow simultaneous targeting of the TEP1, LRIM1 and APL1C promoters by TAL0 (target sites indicated in S4 Table). Transgenic lines PPO6-RFP,3xP3-YFP and Lp-RFP,3xP3-GFP and Vg-GFP,3xP3-RFP were previously described . Promoters and genes were amplified from genomic DNA or cDNA by PCR with primers containing appropriate sites for Goldengate or Gateway cloning. All constructs were verified by sequencing.
To introduce the TEP1r,3xP3-YFP transgene in the background of the TEP1ΔT and TEP1Δct2 mutations , the transgenic line was backcrossed three times to the mutant line. After each backcross, YFP-positive progeny larvae were purified with the COPAS flow cytometer  to retain the transgene. After the last backcross, one leg from 48 male and 48 female mosquitoes kept alive in individual tubes was analyzed by PCR as described  using the Phire Direct Tissue PCR kit (Thermofisher). Mosquitoes showing homozygosity for the TEP1 mutation were pooled to establish a homozygous mutant and heterozygous transgenic line. For experiments, COPAS sorting of this line was used to generate cultures containing 50% non-transgenic mutant control and 50% transgenic mutant mosquitoes. In some cases, non-mutant control mosquitoes with RFP eye fluorescence (such as Vg-GFP,3xP3-RFP) were added to the same culture. On the day of dissection, transgenic and non-transgenic mosquitoes were separated under a fluorescence microscope based on the eye fluorescence of the transgenesis markers. This process ensured identical exposures of all mosquito genotypes to the same growth and environmental conditions.
Knockdown of TEP1 by dsRNA
Allele specific knockdown of TEP1 was performed by injection of dsRNA targeted specifically against TEP1r or TEP1s as previously described . dsRNA was injected into the thorax of one day old female mosquitoes, three days prior to infection. Allele specific knockdown was verified by qRT-PCR. SPCLIP1 RNAi knockdown was performed as described .
Mosquitoes were dissected in PBS, fixed in paraformaldehyde for 20 min, permeabilized in PBS containing 0.1% triton (PBST) for 10 min, blocked in PBST containing 1%BSA (PBSTB) for one hour. Mosquito tissues were incubated with primary antibody (rabbit anti TEP, mouse anti Lipophorin) for at least two hours, washed 3 times and incubated with fluorescent secondary antibody (Alexa488, or Cy3) in PBSTB containing 1μg/μl DAPI. Tissues were washed three times in PBST and mounted on a slide with a drop of Aqua/poly mount (Polysciences). For fat body analysis, mosquitoes were dissected and treated as previously described . Images were collected under a Zeiss LSM 710 confocal microscope.
RNA for RT PCR was extracted from groups of 5–10 mosquitoes. Mosquitoes were collected on ice into 300 μl RNAzol RT (MRC), homogenized with a Precellys homogenizer, with 2 pulses of 20 seconds. RNA was purified on DirectZol RNA columns (Zymo Research) following manufacturer's instructions. RNA was treated with RNAse-free DNAse I (ThermoFisher). Reverse transcription was performed using iScript cDNA Synthesis Kit (Bio-Rad) using 500 μg of RNA. SYBR Green PCR Master Mix, (Applied Biosystems) qPCR reactions were set up on 96 well plates with three technical and three biological repetitions and were run on 7500 Real-time PCR machine (Applied Biosystems).
Western blot analysis
Mosquito hemolymph from 10 mosquitoes was collected by proboscis clipping directly into 20 μl of Laemmli buffer. Samples were heated at 90°C for 2–5 minutes and 2 to 8 μl (depending on the experiment) were loaded on polyacrylamide gels. Rabbit polyclonal antibodies against TEP1, APL1C, LRIM1, PPO2 and Vg were used. Secondary HRP conjugated antibodies were used at 1:15000 dilution. Images were collected on Fusion FX7 scanner (Vilber Lourmat).
Luciferase assay in S2 cells
S2 cells were grown at 23°C in Schneider's medium (Biowest) supplemented with 10% FCS (Invitrogen) and 1% Penicillin/Streptomycin solution (Sigma). Cells were seeded in 24 well plates (Starsted) at 50,000 cells/well one day prior to transfection. Constructs expressing both firefly luciferase and Renilla luciferase were used as reporters. TEP1 promoter was cloned upstream of firefly luciferase. Renilla luciferase under the constitutive actin5c promoter was used as transfection control. Cells were transfected using Effectene (Qiagen) according to manufacturer's instructions. Cells were collected three days after transfection for luciferase activity analysis. Luciferase assay was performed using the Dual-Luciferase Reporter Assay System (Promega) according to manufacturer's instructions. Luciferase activity is depicted as Firefly activity divided by Renilla activity, averaged on three wells transfected with a set of given plasmids.
5'RACE in S2 cells
RNA from S2 cells was extracted using RNAzol RT (MRC) and purified on DirectZol RNA columns (Zymo Research). 5' RACE was performed using First Choice RLM-Race kit (Ambion) according to manufacturer's instructions. Briefly, ligation of specific primers to 5' and 3' ends of the RNA allows the amplification of a PCR product that corresponds to the transcription start site of gene of interest. The resulting PCR product was cloned into CloneJet PCR Cloning Kit (ThermoFisher Scientific) followed by sequencing of several clones.
This project was approved by the French Ministry for Research (agreement #555.01) upon review by its Ethics Committee for Animal Research CREMEAS #35, which approved the research. Experiments were carried out in conformity with the 2010/63/UE European animal bioethics legislation. Our animal care facility received agreement #F67-482-2 from the veterinary services of the region Bas-Rhin (Direction Départementale de la Protection des Populations).
S1 Table. Summary of infections of TEP1-GFP reporter with P. berghei.
Control mosquitoes and TEP1-GFP transgenic mosquitoes were grown together as larvae. Immediately prior to infectious blood feeding mosquitoes were selected according to their GFP expression level separating into two groups with low or high expression. 7 days after infection, oocysts were counted and compared between the three groups. n is the number of analyzed midguts in each condition. p values were calculated for the difference in oocyst numbers between low and high GFP expressing groups, using the non parametric Mann-Whitney t test.
n is the number of analyzed midguts, Prevalence of infection is the number of midguts with at least one parasite out of the total number of midguts. Oocysts and melanized parasites were counted 7 days after infection. p values are from the non parametric Mann-Whitney t-test. Compared groups are marked in bold and are indicated in Fig 4.
n is the number of analyzed midguts, prevalence of infection is the number of midguts with at least one parasite out of the total number of midguts. Oocysts were counted 7 days after infection. P values were calculated using non parametric Mann-Whitney t-test analysis.
S4 Table. Designed TALES and their Repeat-variable di-residues (RVDs).
Taking advantage of the ambiguous recognition of nucleotides by the RVD NS, TAL0 was designed to target TRWSRSBRGGRAWTCCCS, thus targeting the following promoter sites: TGAGGGCAGGGAATCCCC (TEP1), TATCAGGAGGAAATCCCC (LRIM1) and TATCACTGGGAATTCCCG (APL1C).
S1 Fig. Expression of GFP in TEP1-GFP,3xP3-RFP reporter mosquitoes.
a. GFP expression in the proventriculus of a blood fed female. b. GFP expression in proventriculus of a male. c. GFP expression in a blood fed female showing expression in Malpighian tubules (mt) and ovarian duct (od) of a blood fed female 24h after blood feeding. Right panel shows GFP expression in boxed ovary. d. Two transgenic larvae expressing GFP under the TEP1 promoter. Note the strikingly different levels of GFP expression. GFP expression is in green, transgenic marker in red. e. Two live transgenic TEP1-GFP mosquito abdomens showing variable GFP expression.
S2 Fig. Variability in GFP levels in transgenic TEP1-GFP larvae.
100 larvae were analyzed on each indicated day and the level of GFP expression was noted, ranging from no GFP to +++ (highest GFP expression). Shown are 4 independent experiments analyzing four different generations.
S3 Fig. TEP1 levels in transgenic TEP1s;Vg-TEP1r.
a. qPCR analysis of TEP1r mRNA in TEP1s;Vg-TEP1r transgenic mosquitoes expressing TEP1r under control of the Vg promoter. Mosquito RNA was analyzed at different time points after a blood feeding. Expression is relative to RPL19 mRNA in each sample and normalized to time point zero hours after blood feeding. b. Western blot analysis of mosquito whole body (carcasses) and hemolymph showing that there is no increase in TEP1 protein levels in TEP1s;Vg-TEP1r mosquitoes. Control mosquitoes expressed GFP under the Vg promoter (TEP1s;Vg-GFP). PPO2 and actin were used as loading control for hemolymph and carcasses.
S4 Fig. Binding of transgenic TEP1r to ookinetes.
Control mosquitoes expressing TEP1r (left panel), show TEP1 binding (red) to the majority of GFP expressing P. berghei parasites (green). In TEP1 mutant mosquitoes (middle panel) TEP1 does not bind to ookinetes and in mutants over-expressing TEP1r (right panel), transgenic TEP1 is bound to some of the parasites.
S5 Fig. P. berghei infection of mosquitoes expressing transgenic TEP1r in wt background following prior induction by blood feeding.
Compared are transgenic mosquitoes expressing TEP1r or GFP under the Vg promoter. For each mosquito group the un-induced (no prior blood meal) and the induced (blood fed on a non infected mouse 3 days before infection) are compared. Shown are live parasites (green circles) and melanized parasites (black circles) in the midguts of blood fed mosquitoes 7 days after infection. Infection data is given in S2 Table.
S6 Fig. TEP1 promoter architecture.
a. Schematic representation of the 3 kb promoter fragment, indicating the position of potential TATA boxes (yellow), potential NF-κB binding sites (blue) and TALE binding sites (red). Drawing not to scale. b. Four TEP1 promoter fragments fused to a luciferase reporter gene. The position of potential TATA boxes (yellow), potential NF-κB binding sites (blue), TALE binding sites (red), Luciferase gene (light blue) and SV40 term (green) is shown. c. Sequence of the 251bp minimal promoter with TALE binding sites (red) and transcription start site (determined by 5'RACE) indicated by an arrow and 5'UTR. The GGGAATCCC NF-κB binding site is in the TAL0 recognition site indicated by Italic.
S7 Fig. Analysis of the activity of successive truncations of the TEP1 promoter region in S2 cells.
Four different luciferase constructs (described in S3b Fig) were transfected into S2 cells and analyzed for Luciferase activity. For each condition, induction of the NF-κB pathway was triggered by addition of heat killed bacteria to cell medium. Depicted is luciferase activity in non-induced (white) and E. coli challenged (grey) cells. Luciferase activity is normalized to the activity in cells transfected with the full length promoter and uninduced. Shown is the average of three independent experiments. Transfected construct carries firefly luciferase under the control of TEP1 as well as Renilla luciferase under a constitutive promoter which serves as control. Luciferase activity is expressed as firefly luciferase activity divided by Renilla luciferase activity.
S8 Fig. Determining the best activation domain for TALES.
TALEs with the same DNA binding domain (TAL0) but different activation domains were co-transfected into S2 cells together with the Luciferase reporter under the control of the minimal TEP1 promoter fragment. Control (no TAL) were transfected with GFP, TALΔAD has no activation domain and serves as control, yeast GAL4, heat shock factor 1 transcription (HSF) and Herpes virus VP-16 domains were tested. Depicted is luciferase activity in uninduced (white) and induced (grey) cells. Luciferase activity is normalized to the activity in cells transfected with GFP and uninduced. Shown is a representative of at least 3 independent experiments. Error bars depict standard deviation from the mean of three biological repetitions.
S9 Fig. Mutating the NF-κB binding site in the TEP1 promoter abolishes induction by E.coli.
S2 cells were transfected with two different reporters, one with a 250bp fragment of TEP1 promoter carrying an NF-κB binding site, or with the same promoter fragment where the NF-κB binding site was mutated (GGGAATCCCC to CGGAATACCG). Together with the reporter, cells were transfected either with a plasmid encoding GFP (no TAL) or a TAL6-VP16 construct. Depicted is luciferase activity with (grey) or without (white) E. coli challenge. Luciferase activity is normalized to relative to the activity in cells transfected with GFP and without E. coli. Shown is a representative of at least 3 independent experiments. Error bars depict standard deviation from the mean of three biological repetitions.
S1 File. SPCLIP1 silencing abolishes P. berghei melanization in TEP1ΔT; Vg-TEP1r mosquitoes.
S1 Text. Sequences.
Complete sequences of plasmids, as well as promoters and TALE domains that were used in this study.
We thank Elena Levashina for useful scientific discussions and critical reading of the manuscript, and Maëva Roustain for technical assistance.
- Conceived and designed the experiments: GV EM.
- Performed the experiments: GV AKH MS JS EM.
- Analyzed the data: GV AKH EM.
- Contributed reagents/materials/analysis tools: HS JB.
- Wrote the paper: GV EM.
- Contributed interpretation of data for the work: GV EM SAB. Revised work critically for important intellectual content: GV EM SAB. Approved final version to be published: GV EM SAB. Agreement to be accountable for all aspects of the work: GV EM SAB.
- 1. WHO (2015) Malaria Report.
- 2. Harbach RE (1994) Review of the internal classification of the genus Anopheles (Diptera: Culicidae): the foundation for comparative systematics and phylogenetic research. Bull Entomol Res 84: 331–342.
- 3. Kiszewski A, Mellinger A, Spielman A, Malaney P, Sachs SE, et al. (2004) A global index representing the stability of malaria transmission. Am J Trop Med Hyg 70: 486–498. pmid:15155980
- 4. Catteruccia F (2007) Malaria vector control in the third millennium: progress and perspectives of molecular approaches. Pest Manag Sci 63: 634–640. doi: 10.1002/ps.1324. pmid:17373671
- 5. Wang S, Jacobs-Lorena M (2013) Genetic approaches to interfere with malaria transmission by vector mosquitoes. Trends Biotechnol 31: 185–193. doi: 10.1016/j.tibtech.2013.01.001. pmid:23395485
- 6. Mamai W, Lees RS, Maiga H, Gilles JR (2016) Reusing larval rearing water and its effect on development and quality of Anopheles arabiensis mosquitoes. Malar J 15: 169. doi: 10.1186/s12936-016-1227-4. pmid:26984183
- 7. Gato R, Lees RS, Bruzon RY, Companioni A, Menendez Z, et al. (2014) Large indoor cage study of the suppression of stable Aedes aegypti populations by the release of thiotepa-sterilised males. Mem Inst Oswaldo Cruz 109: 365–370. doi: 10.1590/0074-0276130519. pmid:24863972
- 8. Lacroix R, McKemey AR, Raduan N, Kwee Wee L, Hong Ming W, et al. (2012) Open field release of genetically engineered sterile male Aedes aegypti in Malaysia. PLoS One 7: e42771. doi: 10.1371/journal.pone.0042771. pmid:22970102
- 9. Harris AF, McKemey AR, Nimmo D, Curtis Z, Black I, et al. (2012) Successful suppression of a field mosquito population by sustained release of engineered male mosquitoes. Nat Biotechnol 30: 828–830. doi: 10.1038/nbt.2350. pmid:22965050
- 10. Carvalho DO, McKemey AR, Garziera L, Lacroix R, Donnelly CA, et al. (2015) Suppression of a Field Population of Aedes aegypti in Brazil by Sustained Release of Transgenic Male Mosquitoes. PLoS Negl Trop Dis 9: e0003864. doi: 10.1371/journal.pntd.0003864. pmid:26135160
- 11. Burt A (2003) Site-specific selfish genes as tools for the control and genetic engineering of natural populations. Proc Biol Sci 270: 921–928. doi: 10.1098/rspb.2002.2319. pmid:12803906
- 12. Windbichler N, Menichelli M, Papathanos PA, Thyme SB, Li H, et al. (2011) A synthetic homing endonuclease-based gene drive system in the human malaria mosquito. Nature 473: 212–215. doi: 10.1038/nature09937. pmid:21508956
- 13. Sinkins SP, Gould F (2006) Gene drive systems for insect disease vectors. Nat Rev Genet 7: 427–435. doi: 10.1038/nrg1870. pmid:16682981
- 14. Gantz VM, Bier E (2015) Genome editing. The mutagenic chain reaction: a method for converting heterozygous to homozygous mutations. Science 348: 442–444. doi: 10.1126/science.aaa5945. pmid:25908821
- 15. Akbari OS, Bellen HJ, Bier E, Bullock SL, Burt A, et al. (2015) BIOSAFETY. Safeguarding gene drive experiments in the laboratory. Science 349: 927–929. doi: 10.1126/science.aac7932. pmid:26229113
- 16. Gantz VM, Jasinskiene N, Tatarenkova O, Fazekas A, Macias VM, et al. (2015) Highly efficient Cas9-mediated gene drive for population modification of the malaria vector mosquito Anopheles stephensi. Proc Natl Acad Sci U S A 112: E6736–6743. doi: 10.1073/pnas.1521077112. pmid:26598698
- 17. Hammond A, Galizi R, Kyrou K, Simoni A, Siniscalchi C, et al. (2016) A CRISPR-Cas9 gene drive system targeting female reproduction in the malaria mosquito vector Anopheles gambiae. Nat Biotechnol 34: 78–83. doi: 10.1038/nbt.3439. pmid:26641531
- 18. Al-Mashhadani HM, Davidson G, Curtis CF (1980) A genetic study of the susceptibility of Anopheles gambiae to Plasmodium berghei. Trans R Soc Trop Med Hyg 74: 585–594. pmid:7010688
- 19. Blandin S, Shiao SH, Moita LF, Janse CJ, Waters AP, et al. (2004) Complement-like protein TEP1 is a determinant of vectorial capacity in the malaria vector Anopheles gambiae. Cell 116: 661–670. pmid:15006349
- 20. Levashina EA, Moita LF, Blandin S, Vriend G, Lagueux M, et al. (2001) Conserved Role of a Complement-like Protein in Phagocytosis Revealed by dsRNA Knockout in Cultured Cells of the Mosquito, Anopheles gambiae. Cell 104: 709–718. pmid:11257225
- 21. Fraiture M, Baxter RH, Steinert S, Chelliah Y, Frolet C, et al. (2009) Two mosquito LRR proteins function as complement control factors in the TEP1-mediated killing of Plasmodium. Cell Host Microbe 5: 273–284. doi: 10.1016/j.chom.2009.01.005. pmid:19286136
- 22. Povelones M, Waterhouse RM, Kafatos FC, Christophides GK (2009) Leucine-rich repeat protein complex activates mosquito complement in defense against Plasmodium parasites. Science 324: 258–261. doi: 10.1126/science.1171400. pmid:19264986
- 23. Molina-Cruz A, Garver LS, Alabaster A, Bangiolo L, Haile A, et al. (2013) The human malaria parasite Pfs47 gene mediates evasion of the mosquito immune system. Science 340: 984–987. doi: 10.1126/science.1235264. pmid:23661646
- 24. Molina-Cruz A, Canepa GE, Kamath N, Pavlovic NV, Mu J, et al. (2015) Plasmodium evasion of mosquito immunity and global malaria transmission: The lock-and-key theory. Proc Natl Acad Sci U S A 112: 15178–15183. doi: 10.1073/pnas.1520426112. pmid:26598665
- 25. Blandin SA, Wang-Sattler R, Lamacchia M, Gagneur J, Lycett G, et al. (2009) Dissecting the genetic basis of resistance to malaria parasites in Anopheles gambiae. Science 326: 147–150. doi: 10.1126/science.1175241. pmid:19797663
- 26. Collins FH, Sakai RK, Vernick KD, Paskewitz S, Seeley DC, et al. (1986) Genetic selection of a Plasmodium-refractory strain of the malaria vector Anopheles gambiae. Science 234: 607–610. pmid:3532325
- 27. Smidler AL, Terenzi O, Soichot J, Levashina EA, Marois E (2013) Targeted mutagenesis in the malaria mosquito using TALE nucleases. PLoS One 8: e74511. doi: 10.1371/journal.pone.0074511. pmid:23977401
- 28. Tang H (2009) Regulation and function of the melanization reaction in Drosophila. Fly (Austin) 3: 105–111.
- 29. Kumar S, Christophides GK, Cantera R, Charles B, Han YS, et al. (2003) The role of reactive oxygen species on Plasmodium melanotic encapsulation in Anopheles gambiae. Proc Natl Acad Sci U S A 100: 14139–14144. doi: 10.1073/pnas.2036262100. pmid:14623973
- 30. Volz J, Osta MA, Kafatos FC, Muller HM (2005) The roles of two clip domain serine proteases in innate immune responses of the malaria vector Anopheles gambiae. J Biol Chem 280: 40161–40168. doi: 10.1074/jbc.M506191200. pmid:16188883
- 31. Volz J, Muller HM, Zdanowicz A, Kafatos FC, Osta MA (2006) A genetic module regulates the melanization response of Anopheles to Plasmodium. Cell Microbiol 8: 1392–1405. doi: 10.1111/j.1462-5822.2006.00718.x. pmid:16922859
- 32. Warr E, Lambrechts L, Koella JC, Bourgouin C, Dimopoulos G (2006) Anopheles gambiae immune responses to Sephadex beads: involvement of anti-Plasmodium factors in regulating melanization. Insect Biochem Mol Biol 36: 769–778. doi: 10.1016/j.ibmb.2006.07.006. pmid:17027843
- 33. Shiao SH, Whitten MM, Zachary D, Hoffmann JA, Levashina EA (2006) Fz2 and cdc42 mediate melanization and actin polymerization but are dispensable for Plasmodium killing in the mosquito midgut. PLoS Pathog 2: e133. doi: 10.1371/journal.ppat.0020133. pmid:17196037
- 34. Volohonsky G, Terenzi O, Soichot J, Naujoks DA, Nolan T, et al. (2015) Tools for Anopheles gambiae Transgenesis. G3 (Bethesda) 5: 1151–1163.
- 35. Frolet C, Thoma M, Blandin S, Hoffmann JA, Levashina EA (2006) Boosting NF-kappaB-dependent basal immunity of Anopheles gambiae aborts development of Plasmodium berghei. Immunity 25: 677–685. doi: 10.1016/j.immuni.2006.08.019. pmid:17045818
- 36. Nirmala X, Marinotti O, James AA (2005) The accumulation of specific mRNAs following multiple blood meals in Anopheles gambiae. Insect Mol Biol 14: 95–103. doi: 10.1111/j.1365-2583.2005.00535.x. pmid:15663779
- 37. Rono MK, Whitten MM, Oulad-Abdelghani M, Levashina EA, Marois E (2010) The major yolk protein vitellogenin interferes with the anti-plasmodium response in the malaria mosquito Anopheles gambiae. PLoS Biol 8: e1000434. doi: 10.1371/journal.pbio.1000434. pmid:20652016
- 38. Baxter RH, Steinert S, Chelliah Y, Volohonsky G, Levashina EA, et al. (2010) A heterodimeric complex of the LRR proteins LRIM1 and APL1C regulates complement-like immunity in Anopheles gambiae. Proc Natl Acad Sci U S A 107: 16817–16822. doi: 10.1073/pnas.1010575107. pmid:20826443
- 39. Povelones M, Bhagavatula L, Yassine H, Tan LA, Upton LM, et al. (2013) The CLIP-domain serine protease homolog SPCLIP1 regulates complement recruitment to microbial surfaces in the malaria mosquito Anopheles gambiae. PLoS Pathog 9: e1003623. doi: 10.1371/journal.ppat.1003623. pmid:24039584
- 40. Yassine H, Kamareddine L, Chamat S, Christophides GK, Osta MA (2014) A serine protease homolog negatively regulates TEP1 consumption in systemic infections of the malaria vector Anopheles gambiae. J Innate Immun 6: 806–818. doi: 10.1159/000363296. pmid:25012124
- 41. Boch J, Scholze H, Schornack S, Landgraf A, Hahn S, et al. (2009) Breaking the code of DNA binding specificity of TAL-type III effectors. Science 326: 1509–1512. doi: 10.1126/science.1178811. pmid:19933107
- 42. Geissler R, Scholze H, Hahn S, Streubel J, Bonas U, et al. (2011) Transcriptional activators of human genes with programmable DNA-specificity. PLoS One 6: e19509. doi: 10.1371/journal.pone.0019509. pmid:21625585
- 43. Joung JK, Sander JD (2013) TALENs: a widely applicable technology for targeted genome editing. Nat Rev Mol Cell Biol 14: 49–55. doi: 10.1038/nrm3486. pmid:23169466
- 44. Kay S, Hahn S, Marois E, Hause G, Bonas U (2007) A bacterial effector acts as a plant transcription factor and induces a cell size regulator. Science 318: 648–651. doi: 10.1126/science.1144956. pmid:17962565
- 45. Kay S, Hahn S, Marois E, Wieduwild R, Bonas U (2009) Detailed analysis of the DNA recognition motifs of the Xanthomonas type III effectors AvrBs3 and AvrBs3Deltarep16. Plant J 59: 859–871. doi: 10.1111/j.1365-313X.2009.03922.x. pmid:19473322
- 46. Rodrigues J, Brayner FA, Alves LC, Dixit R, Barillas-Mury C (2010) Hemocyte differentiation mediates innate immune memory in Anopheles gambiae mosquitoes. Science 329: 1353–1355. doi: 10.1126/science.1190689. pmid:20829487
- 47. Baton LA, Robertson A, Warr E, Strand MR, Dimopoulos G (2009) Genome-wide transcriptomic profiling of Anopheles gambiae hemocytes reveals pathogen-specific signatures upon bacterial challenge and Plasmodium berghei infection. BMC Genomics 10: 257. doi: 10.1186/1471-2164-10-257. pmid:19500340
- 48. Pinto SB, Lombardo F, Koutsos AC, Waterhouse RM, McKay K, et al. (2009) Discovery of Plasmodium modulators by genome-wide analysis of circulating hemocytes in Anopheles gambiae. Proc Natl Acad Sci U S A 106: 21270–21275. doi: 10.1073/pnas.0909463106. pmid:19940242
- 49. Castillo JC, Robertson AE, Strand MR (2006) Characterization of hemocytes from the mosquitoes Anopheles gambiae and Aedes aegypti. Insect Biochem Mol Biol 36: 891–903. doi: 10.1016/j.ibmb.2006.08.010. pmid:17098164
- 50. Imler JL, Bulet P (2005) Antimicrobial peptides in Drosophila: structures, activities and gene regulation. Chem Immunol Allergy 86: 1–21. doi: 10.1159/000086648. pmid:15976485
- 51. Marinotti O, Calvo E, Nguyen QK, Dissanayake S, Ribeiro JM, et al. (2006) Genome-wide analysis of gene expression in adult Anopheles gambiae. Insect Mol Biol 15: 1–12. doi: 10.1111/j.1365-2583.2006.00610.x. pmid:16469063
- 52. Bou Aoun R, Hetru C, Troxler L, Doucet D, Ferrandon D, et al. (2011) Analysis of thioester-containing proteins during the innate immune response of Drosophila melanogaster. J Innate Immun 3: 52–64. doi: 10.1159/000321554. pmid:21063077
- 53. Alper CA, Johnson AM, Birtch AG, Moore FD (1969) Human C3: evidence for teh liver as the primary site of synthesis. Science 163: 286–288. pmid:4883617
- 54. Fey G, Domdey H, Wiebauer K, Whitehead AS, Odink K (1984) Structure and Expression of the C3 gene. In: Müller-Eberhard HJ, Miescher PA, editors. Complement. Berlin Heidelberg New York Tokyo: Springer.
- 55. Warr E, Aguilar R, Dong Y, Mahairaki V, Dimopoulos G (2007) Spatial and sex-specific dissection of the Anopheles gambiae midgut transcriptome. BMC Genomics 8: 37. doi: 10.1186/1471-2164-8-37. pmid:17261194
- 56. Hao Z, Kasumba I, Aksoy S (2003) Proventriculus (cardia) plays a crucial role in immunity in tsetse fly (Diptera: Glossinidiae). Insect Biochem Mol Biol 33: 1155–1164. pmid:14563366
- 57. Neira Oviedo M, Vanekeris L, Corena-McLeod MD, Linser PJ (2008) A microarray-based analysis of transcriptional compartmentalization in the alimentary canal of Anopheles gambiae (Diptera: Culicidae) larvae. Insect Mol Biol 17: 61–72. doi: 10.1111/j.1365-2583.2008.00779.x. pmid:18237285
- 58. Moita LF, Wang-Sattler R, Michel K, Zimmermann T, Blandin S, et al. (2005) In vivo identification of novel regulators and conserved pathways of phagocytosis in A. gambiae. Immunity 23: 65–73. doi: 10.1016/j.immuni.2005.05.006. pmid:16039580
- 59. Blandin SA, Marois E, Levashina EA (2008) Antimalarial responses in Anopheles gambiae: from a complement-like protein to a complement-like pathway. Cell Host Microbe 3: 364–374. doi: 10.1016/j.chom.2008.05.007. pmid:18541213
- 60. Franke-Fayard B, Trueman H, Ramesar J, Mendoza J, van der Keur M, et al. (2004) A Plasmodium berghei reference line that constitutively expresses GFP at a high level throughout the complete life cycle. Mol Biochem Parasitol 137: 23–33. doi: 10.1016/j.molbiopara.2004.04.007. pmid:15279948
- 61. Marois E, Scali C, Soichot J, Kappler C, Levashina EA, et al. (2012) High-throughput sorting of mosquito larvae for laboratory studies and for future vector control interventions. Malar J 11: 302. doi: 10.1186/1475-2875-11-302. pmid:22929810
- 62. Dong Y, Aguilar R, Xi Z, Warr E, Mongin E, et al. (2006) Anopheles gambiae immune responses to human and rodent Plasmodium parasite species. PLoS Pathog 2: e52. doi: 10.1371/journal.ppat.0020052. pmid:16789837
- 63. Barillas-Mury C, Han YS, Seeley D, Kafatos FC (1999) Anopheles gambiae Ag-STAT, a new insect member of the STAT family, is activated in response to bacterial infection. EMBO J 18: 959–967. doi: 10.1093/emboj/18.4.959. pmid:10022838