Immune responses mounted by the malaria vector Anopheles gambiae are largely regulated by the Toll and Imd (immune deficiency) pathways via the NF-kappaB transcription factors Rel1 and Rel2, which are controlled by the negative regulators Cactus and Caspar, respectively. Rel1- and Rel2-dependent transcription in A. gambiae has been shown to be particularly critical to the mosquito's ability to manage infection with the rodent malaria parasite Plasmodium berghei. Using RNA interference to deplete the negative regulators of these pathways, we found that Rel2 controls resistance of A. gambiae to the human malaria parasite Plasmodium falciparum, whereas Rel 1 activation reduced infection levels. The universal relevance of this defense system across Anopheles species was established by showing that caspar silencing also prevents the development of P. falciparum in the major malaria vectors of Asia and South America, A. stephensi and A. albimanus, respectively. Parallel studies suggest that while Imd pathway activation is most effective against P. falciparum, the Toll pathway is most efficient against P. berghei, highlighting a significant discrepancy between the human pathogen and its rodent model. High throughput gene expression analyses identified a plethora of genes regulated by the activation of the two Rel factors and revealed that the Toll pathway played a more diverse role in mosquito biology than the Imd pathway, which was more immunity-specific. Further analyses of key anti-Plasmodium factors suggest they may be responsible for the Imd pathway–mediated resistance phenotype. Additionally, we found that the fitness cost caused by Rel2 activation through caspar gene silencing was undetectable in sugar-fed, blood-fed, and P. falciparum-infected female A. gambiae, while activation of the Toll pathway's Rel1 had a major impact. This study describes for the first time a single gene that influences an immune mechanism that is able to abort development of P. falciparum in Anopheline species. Further, this study addresses aspects of the molecular, evolutionary, and physiological consequences of the observed phenotype. These findings have implications for malaria control since broad-spectrum immune activation in diverse anopheline species offers a viable and strategic approach to develop novel malaria control methods worldwide.
The relationship between malaria parasites and the mosquitoes that transmit them to humans comprises complex molecular interactions including mosquito immune responses. Anopheles can mount potent anti-Plasmodium immune responses; we show here that the gene caspar, which encodes a negative regulator of the immune signaling pathway Imd, controls mosquito resistance to the human malaria parasite. Silencing of this Imd pathway regulator results in complete resistance to human Plasmodium in three divergent Anopheline malaria vector species, yet does not cause complete resistance to a rodent Plasmodium species, indicating conservation of defense function among mosquito but not diverse parasite species. We also identify a panel of genes that are transcriptionally regulated by silencing of the caspar gene. Some of these genes contribute directly to parasite resistance. Finally, we show that the transient immune activation that renders mosquitoes resistant to the human malaria parasite has little to no effect on mosquito fitness as a measure of survival or fecundity under laboratory conditions. In sum, this study shows that the mosquito's immune pathway, Imd, can regulate resistance to Plasmodium through immune responses that entail several known anti-Plasmodium genes.
Citation: Garver LS, Dong Y, Dimopoulos G (2009) Caspar Controls Resistance to Plasmodium falciparum in Diverse Anopheline Species. PLoS Pathog 5(3): e1000335. doi:10.1371/journal.ppat.1000335
Editor: José M. C. Ribeiro, National Institute of Allergy and Infectious Diseases, United States of America
Received: November 24, 2008; Accepted: February 12, 2009; Published: March 13, 2009
Copyright: © 2009 Garver 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.
Funding: This material is based upon work supported under a National Science Foundation Graduate Research Fellowship (LSG). This work is also supported by National Institutes of Health/National Institute for Allergy and Infectious Disease grant 1R01AI061576-01A1, the United Nations Development Program/World Bank/World Health Organization Special Program for Research and Training in Tropical Diseases, The Ellison Medical Foundation, the Johns Hopkins School of Public Health, the Johns Hopkins Malaria Research Institute, and the Bloomberg Foundation.
Competing interests: The authors have declared that no competing interests exist.
The innate immune system of the African malaria vector, Anopheles gambiae, is the mosquito's main line of defense against Plasmodium parasites and is engaged at multiple stages of parasite infection ,. As part of this defense, two major signaling pathways, Toll and Imd, transduce the pathogen recognition signal to activate nuclear translocation of the NF-kappaB Rel family transcription factors, which transcriptionally induce effector genes such as antimicrobial peptides . Previous studies have implicated both pathways in the modulation of the mosquito's susceptibility to the rodent malaria parasite P. berghei, while a variety of immune effector genes have been shown to mediate the killing of the human pathogen P. falciparum –. Interestingly, defense responses to these two Plasmodium species have been shown to be quite different, as exemplified by the identification of several parasite species-specific anti-Plasmodium genes ,.
In A. gambiae, Rel1 (previously Gambif1) is controlled by the Toll pathway and is an analog of the D. melanogaster Dif, while Rel2 is controlled by the Imd pathway and is the ortholog of the D. melanogaster Relish , –. In both species, the negative regulator of the Toll pathway, Cactus, is bound to Dif/Rel1 under naïve conditions, sequestering the transcription factor in the cytoplasm ,. When Toll is activated, the signal is transmitted through adaptor proteins triggering phosphorylation of Cactus which tags it for degradation. Destruction of Cactus frees Dif/Rel1, which can then enter the nucleus and initiate transcription .
The activity of the Imd Rel factor (Relish/Rel2) is held in check by its own inhibitory domains (ankyrin repeats) which can be cleaved by Dredd, a caspase-8 homolog, to cause activation ,. Regulation of Relish has been shown by Kim and colleagues to be negatively controlled by Caspar, a homolog of the mammalian Fas-associating factor . After observing an increased resistance to Gram negative bacterial exposure and constitutive production of the antimicrobial peptide Diptericin, they determined that Caspar is a negative regulator specific to the Imd pathway that inhibits nuclear localization of Relish by blocking Dredd from cleaving Relish under naïve conditions . Since this is the first and, so far, only study of Caspar, our knowledge of the exact nature and extent of Caspar's inhibitory role is limited.
A variety of A. gambiae immune-responsive genes have been identified via gene expression profiling in which mosquitoes infected with bacteria, fungi or malaria parasites have been compared to uninfected controls , –. Assays comparing bacteria-challenged and naïve Rel1- or Rel2-depleted mosquitoes have identified both Toll and Imd pathway-regulated immune genes ,. Many of these pathway-regulated genes, such as TEP1 (thioester-containing protein 1) and LRIM1, have been shown to play key roles in parasite elimination ,,. What is unknown about some of these immune pathways and effectors is the role they play during P. falciparum infection and whether they work together or independently while exerting their anti-parasitic action. The complex network of pathogen detection, signal transduction and effector action that ultimately leads to parasite destruction is of utmost interest for the development of vector-based malaria control strategies.
Over 40 Anopheles mosquito species act as malaria vectors throughout the world, encountering different environments, food sources, microbial exposures and parasite strains, all of which could impose evolutionary pressures on the insect immune system ,. A pressing question is whether the anti-Plasmodium mechanisms are common or unique among the different Anopheles species. This is particularly interesting for anti-Plasmodium mechanisms based on immune responses because certain elements of an integrated immune system are conserved while others are highly divergent ,. Here we have for the first time addressed the role of the Toll and Imd immune signaling pathways in mosquito defense against the human malaria parasite P. falciparum not only in A. gambiae but also in A. stephensi and A. albimanus to assess the potential universality of these defense mechanisms. Towards this we have also directly compared the implication of these pathways in the defense against different malaria parasite species.
A finely tuned balance between the capacity of the mosquito's immune system to kill malaria parasites and the impact of Plasmodium infection on mosquito fitness exist. A negative correlation has been established between fitness and immune induction but only under chronic conditions which is not the case during transient immune pathway activation . To gain a better insight of the fitness cost of a transient activation of a highly potent immune pathway-mediated anti-Plasmodium defense on the mosquito's fitness we have looked at how a cactus- or caspar-silencing-based immune activation affect the ability of mosquitoes to survive and reproduce.
These novel findings have important implications for understanding molecular and evolutionary components of mosquito immunity to the Plasmodium parasite and for the development of vector-based immune-mediated malaria control strategies.
A. gambiae Caspar is a negative regulator of the Imd pathway–controlled Rel2
The Anopheles cactus gene was previously identified through a comparative immunogenomics study of the Drosophila and Anopheles immune systems and has been functionally confirmed as a negative regulator of Rel1 ,. Sequence comparison between the putative A. gambiae caspar and D. melanogaster caspar showed that the mosquito protein sequence shares 43% identity and 59% similarity. Four conserved sequence regions occur similarly in Anopheles Caspar as they do in both Drosophila Caspar and human FAF1: the Fas-associating region, the DED-interacting region, the ubiquitin-associated domain (UAS) and the ubiquitin-like domain. Fas-associating regions between the two insects' Caspar amino acid sequences were 46% similar, the DED-interacting region, UAS and Ubx domains share 55%, 78% and 81% similarity, respectively (Figure 1A).
(A) Domain comparison between Drosophila Caspar (upper diagram) and Anopheles Caspar (lower diagram). The horizontal black bar represents the amino acid sequence; black, gray, and white boxes indicate four functional domains of Caspar. Percentage indicates the degree of sequence similarity. DED, death effector domain; UAS, ubiquitin-associated domain; Ubx, ubiquitin-like domain. (B) Silencing efficiency of caspar, cactus, rel1, and rel2. Bars represent the percent knockdown compared to controls treated with dsRNA against GFP as determined by qRT-PCR. Error bars represent standard deviation of three independent assays. (C) Expression of genes following single or double knockdown in adults. Bars represent fold change in expression compared to GFP dsRNA–treated controls. Horizontal gray line represents baseline expression (i.e., a 1∶1 expression ratio between control and silenced samples). Silencing treatment is indicated by the legend. Error bars represent standard deviation across three biological replicates. Cec1, cecropin1; Def1, defensin1; Gam, gambicin; Cec3, cecropin3; A9, ClipA9; CathD, cathepsinD.
To investigate potential functional conservation we combined an RNAi (RNA interference) -mediated gene-silencing approach with expression analyses of putative Imd pathway immune markers. A dsRNA targeting caspar or cactus was used to silence the respective mRNA transcript in adult female mosquitoes. The average silencing efficiency was 79% for caspar and 75% for cactus, while rel1 and rel2 displayed significantly lower gene-silencing efficiencies of 62% and 55%, respectively, as previously reported (Figure 1B) . The resulting effects on Imd pathway-dependent gene expression were then quantified using quantitative real-time PCR (qRT-PCR) amplification of a panel of antimicrobial peptides (AMPs) previously predicted as Toll or Imd pathway marker genes as well as two genes identified via microarray transcription analyses as regulated by one pathway but not the other ,. All AMPs showed moderate induction upon Caspar depletion within a 2- to 5-fold range, suggesting that the Anopheles caspar is functionally conserved to the Drosophila caspar (Figure 1C and Table S1B). To further confirm this relationship and specifically link the Caspar-mediated induction of immune markers to the Rel2 transcription factor, a double gene-silencing assay was performed in which the effect of Caspar depletion was reversed through simultaneous Rel2 depletion. A similar strategy was used for Cactus and Rel1 to ensure consistency. For almost all markers tested, double knockdown reversed the transcriptional increase observed for single knockdown of either caspar or cactus (Figure 1C), suggesting that Caspar has an influence on Rel2 that affects transcription initiation of key immune genes. A complete reversal of the effects of caspar or cactus silencing through rel1 and rel2 silencing would not be expected, given the transient and partial efficiency of RNAi-mediated protein depletion.
Resistance of mosquitoes to either the human or rodent Plasmodium parasites is differentially dependent on the Toll and Imd pathways
To investigate the role of these negative regulators in controlling mosquito permissiveness to either the human malaria parasite P. falciparum or the rodent malaria parasite P. berghei, we depleted female A. gambiae of Cactus and Caspar and then fed them on either P. falciparum-infected blood through a membrane or on a P. berghei infected mouse. Infection levels were compared between the gene-silenced mosquitoes and the GFP dsRNA-treated controls by counting oocysts in the midgut tissue. Strikingly, of the 94 mosquitoes tested in three independent biological assays, only 15 Caspar-depleted mosquitoes (15.5%) allowed a small number of P. falciparum to develop to the oocyst stage, as compared to 61.3% of the Cactus-depleted and 65.4% of the control GFP dsRNA-treated mosquitoes (Figure 2A, left panel). While the median number of oocysts per gut was 0 in Caspar-depleted mosquitoes, there were still several individuals with low levels of infection. This is likely to have resulted from incomplete gene silencing in these few individuals, which still displayed an unusually low infection level with a median of 1 oocyst (mean = 1.25 oocysts) (Figure 2A, right panel). This is in stark contrast to that of GFP dsRNA-treated mosquitoes, which had a median infection intensity of 9 P. falciparum oocysts per midgut (mean = 21 oocysts) (Figure 2A, right panel). The Cactus-depleted mosquitoes had a median intensity of infection of 2 oocysts (mean = 8 oocysts) which was just less than one-third of that detected in the control mosquitoes, suggesting that the Toll pathway-controlled Rel1 also exerts an anti-P. falciparum effect but not nearly as potent as that of Rel2 (Figure 2A, right panel).
Prevalence and infection intensity as a measure of P. falciparum oocysts in A. gambiae (A), P. berghei oocysts in A. gambiae (B), P. falciparum oocysts in A. albimanus (C), and in A. stephensi (D). For all, the left panel indicates infection prevalence where the bars represent the total population of mosquitoes examined. The filled portion of the bars indicates the proportion of mosquito midguts that stained positive for at least one oocyst; the open portion of the bar indicates the proportion of midguts that were uninfected. The right panel indicates intensity of infection where blue squares represent individual midgut oocyst counts in mosquitoes receiving RNAi treatment against the given genes; the red bars represent the median number of oocysts per midgut, and the black bars indicate the 95% confidence interval.
Remarkably, experiments with the rodent P. berghei parasite yielded the reverse phenotype: caspar silencing had a degree of impact on oocyst development (over 50% reduction) but it was cactus silencing that caused a drastic reduction in infection intensity although prevalence was comparable among all groups (Figure 2B). This is in agreement with the phenotype observed by Frolet and colleagues and contributes to an emerging hypothesis that some anti-Plasmodium mechanisms, including those utilizing the immune system, show different rates of success when tested comparatively against both P. berghei and P. falciparum ,.
Caspar's effect on P. falciparum is conserved among three Anopheles species
Bearing in mind that species specificities exist not just within Plasmodium but also within Anopheles, we were concerned about the possibility that different mosquito malaria vector species use different molecules and/or mechanisms to contain Plasmodium infections. We investigated the conservation of the anti-P. falciparum phenotype inflicted by caspar silencing by replicating silencing and infection assays in two additional anopheline species. Specifically, we looked at caspar and cactus silencing in Anopheles albimanus, a South American vector, and Anopheles stephensi, an Asian vector. These species were chosen for their status as major malaria vectors in separate geographical areas and their relatedness to A. gambiae. A. stephensi belongs to the same sub-genus as A. gambiae (Cellia) yet distinctly branches from the A. gambiae species complex while A. albimanus belongs to a different sub-genus (Nyssorhynchus) and is distinctly separated from A. gambiae in phylogenic trees generated using single copy, ribosomal and mitochondrial sequences as well as those based on morphological characteristics –. Comparisons of these three species provided insight on the conservation of anti-Plasmodium defenses between mosquitoes that are separated both spatially and evolutionarily.
Degenerate primers were used to identify species-specific caspar and cactus sequences for generation of dsRNA. Using these specific dsRNAs and the same gene-silencing and P. falciparum infection protocol used for A. gambiae, we again observed that caspar silencing causes near-refractoriness. Since the phenotype of these mosquito species mirrored that of A. gambiae, we hypothesize that caspar silencing activates a conserved mechanism for P. falciparum inhibition, consistent with its proposed position in the Imd pathway . dsGFP-treated controls for A. stephensi and A. albimanus exhibited median infection intensities of 6 and 4 oocysts per gut, respectively (means for both = 6 oocysts), while the caspar-silenced mosquitoes from each group had a median of 1 oocyst per gut (means ≤1). The effect of cactus silencing seems more pronounced in A. albimanus, showing a 75% reduction compared to controls, while cactus-silencing in A. stephensi results in a 50% reduction in median number of oocysts per gut.
Molecular analysis suggests that the Imd pathway is highly regulated and influences several anti-Plasmodium effectors
The complexity of an immune response that is more active against one Plasmodium species than another and is conserved among Anopheles species spurred deeper investigation into the molecular outcome of caspar silencing. Identification of molecules affected by caspar silencing would provide insight into how the Caspar-driven phenotype is produced. Towards this we investigated the transcriptional influences of caspar and cactus silencing via a genome-wide comparative transcriptome analysis between Cactus- and Caspar-depleted adult female mosquitoes and control mosquitoes. The robustness of the resulting microarray gene expression data was validated by real-time quantitative PCR (Tables S1A and S1B; Figure S1A and S1B). In total, 588 (472 induced and 116 repressed) genes were significantly regulated upon Cactus depletion and only 116 (61 induced and 55 repressed) were regulated in response to Caspar depletion (Figure 3A and 3B and Tables S3 and S4). In both cases, the majority of the regulated genes belonged to a diverse or unknown functional group; however, there were several remarkable patterns that emerged with regard to other groups of genes (Figure 3A).
(A) Graph indicating functional group distribution of genes regulated by cactus and caspar silencing. For both upper (Cactus) and lower (Caspar) diagrams, colored sections of graphs correspond to the number of genes either up-regulated (right of zero) or down-regulated (left of zero) for the given functional group (see legend). Unk, unknown; Div, diverse; R/T/T, replication/transcription/translation; Met, metabolism; Trp, transport; C/S, cytoskeletal/structure; Rdx/St, redox/stress; Prot, proteolysis and digestion; CSR, chemosensory; Imm, immunity. Functional groups were predicted using Gene Ontology terms . (B) Venn diagram indicating comparative gene regulation between the two treatment groups. The blue and yellow circles represent the gene expression profiles of the cactus- and caspar-silenced mosquitoes, respectively, with the overlapping region (green) representing genes that were regulated by both treatments. Numbers with upward-pointing arrows indicate the number of induced genes, numbers with downward-pointing arrows indicate the number of repressed genes, and the single number with one downward-facing and one upward-facing arrow represents the one gene that was enriched after cactus silencing and repressed after caspar silencing. (C) Temporal expression analysis of anti-Plasmodium gene after Caspar depletion. Bars reflect fold change in expression of the indicated gene at 6, 12, 24, and 48 hours after injection of dsRNA against caspar. Fold change is determined by real-time quantitative PCR comparison to GFP dsRNA–treated controls. Horizontal gray line represents baseline expression (i.e., a 1∶1 expression ratio between control and silenced samples), and error bars indicate standard deviation among three biological replicates. P-values were ≤.05 for: FBN9 at 12 and 48 h.p.i.; TEP1 at 48 h.p.i.; LRRD9 at 6, 24, and 48 h.p.i. Other time points are indicative of trends but did not reach statistical significance among three replicates.
The activation of Rel1 via Cactus depletion induced the transcription of 84 genes involved in replication, transcription and translation. The next most-represented functional groups were immunity, redox/stress responses and metabolism. Caspar-depleted mosquitoes also displayed an elevated expression of genes involved in immunity, redox/stress and replication, transcription and translation. Immune genes regulated by either silencing treatment are outlined in Table S2; description of individual genes of interest regulated by these treatments can be found in Text S1. Of note is that several key anti-Plasmodium genes such as TEP1, LRRD7 (leucine rich repeat domain protein 7) (also known as APL2), and those encoding several FBNs, CLIP domain serine proteases and anti-microbial peptides were regulated by silencing either regulator ,,. Since the microarray depicted only a single time point (3 days post-silencing) and tight temporal regulation of immune genes has been reported , we focused more specifically on the transcriptional regulation of genes encoding three key anti-Plasmodium factors, FBN9 (fibrinogen immunolectin 9), TEP1 and LRRD7, at 6, 12, 24 and 48 hours post caspar dsRNA injection (h.p.i.) to gain a better insight on the temporal nature of this response. Results of these experiments show clearly that these genes are regulated at the transcriptional level by caspar silencing and that this regulation is complex and variable among genes. FBN9 exhibited drastic up-regulation at 6 h.p.i. and its transcripts began to wane as time progresses to reach almost baseline levels (as determined by dsGFP-injected controls) at 24 and 48 hours (Figure 3C, left panel). TEP1 had the opposite expression phenotype where mRNA abundance was still at a baseline level at 6 h.p.i. but climbed incrementally through 24 hours and remained above the baseline level at 48 h.p.i. (Figure 3C, middle panel). LRRD7 followed a similar pattern as FBN9 but with a time lag: the spike in LRRD7 transcript abundance occurred at 12 h.p.i. and began to wane, although expression was still enhanced compared to dsGFP controls even at 48 h.p.i. (Figure 3C, right panel).
To ensure that the transcriptional immune response we observed at the mRNA level was tied to the lack of oocyst development in caspar-silenced mosquitoes, we designed assays to test whether TEP1, FBN9 and LRRD7 are indeed part of the caspar silencing–mediated anti-Plasmodium mechanism. Each of these three genes was silenced independently as well as together with caspar in A. gambiae females which were then infected with P. falciparum. Oocyst counts from the midguts of these mosquitoes are shown in Figure 4. When TEP1 was silenced alone a median of 42 oocysts would develop while concurrent silencing with caspar resulted in 31 oocysts. A median of 27 oocysts developed following FBN9 silencing alone, 23 oocysts when co-silenced with caspar while LRRD7 silencing permitted a median of 69 oocysts which was muted to 42 with caspar silencing. Compared to the dsGFP-treated median infection of 18 oocysts and the caspar-silenced median of 1, each effector significantly reverses the refractoriness conferred by caspar silencing; however, the infections were not as heavy as those that resulted from silencing of any factor alone. We also observe that co-silencing two factors, FBN9 and TEP1, together with caspar did slightly increase infection intensity compared to either the TEP1+caspar or FBN9+caspar group (median = 39 oocysts).
Blue squares represent individual oocyst counts following the indicated RNAi treatment; horizontal red bars represent median number of oocysts per gut, and black bars represent the 95% confidence interval. Assays represent three independent biological replicates and were subject to Mann-Whitney statistical tests. P-values appear below each treatment and refer to that treatment compared to the GFP control. Cpr, Caspar.
Caspar silencing does not impact mosquito fitness
Given the number of genes and variety of functional gene groups that displayed transcriptional induction or repression after Caspar or Cactus depletion (Figure 3), we hypothesized that these P. falciparum-resistant mosquitoes might display a reduced level of fitness. Studies of the trade-offs between lifespan and immune defense have shown that mounting an immune response accelerates aging in insects; more specifically, chronic and sustained but not acute and transient Relish (Rel2)-dependent immune signaling reduces the lifespan of D. melanogaster ,.
The kinetics of RNAi-mediated gene silencing suggest that pathway induction achieved through silencing of negative regulators would persist for a certain period of time and then diminish over time as the dsRNAs are degraded. Furthermore, our study and that of Frolet et al. suggest that a molecular boosting of basal immunity, prior to infection via pathway activation, causes a different profile of immune gene transcription than persistent infection does . Since the impact of this type of pathway activation on parameters that determine fitness is currently unknown, we asked whether our strategy for immune induction could influence mosquito survival and fecundity under laboratory conditions.
Both fitness measures were assessed in A. gambiae females that had been treated with either dsRNA against cactus or caspar or control GFP dsRNA. Non-injected mosquitoes were also monitored to account for injury-related effects. All groups were tested under three different conditions with regard to nutrition and infection status. Mosquitoes were maintained according to one of three conditions: 1. provision of 10% sucrose throughout the duration of life; 2. given a single naïve blood meal followed by sucrose provision; or 3. given a single P. falciparum-laden blood meal followed by sucrose provision. Cactus-depleted mosquitoes given only sucrose showed a slightly impaired survival rate; this was ameliorated by provision of a blood meal but was exacerbated by provision of an infectious blood meal. In stark contrast, Caspar-depleted mosquitoes, regardless of nutritional or infectious status, displayed a similar survival rate to the GFP dsRNA-treated controls and non-injected controls. As expected, non-injected mosquitoes tended to fare better than all injected mosquitoes though not significantly (Figure 5A–5C). The number of eggs laid per female and hatch rates of those eggs were also similar between non-injected controls, GFP dsRNA-treated controls and mosquitoes treated with caspar dsRNA while a quite significant decrease in both measures was observable in the cactus-silenced group (Figure 5D).
(A–C) Longevity: Symbols represent the percent of surviving mosquitoes after RNAi-mediated silencing of genes: Caspar (red squares) or Cactus (green triangles); GFP dsRNA treated control (black diamonds), the non-injected control is indicated by the blue circles. The error bars represent the standard deviation for three independent assays. (A) Mosquitoes maintained on 10% sucrose solution; (B) Mosquitoes given a single naïve blood meal via membrane and maintained on 10% sucrose subsequently; (C) Mosquitoes given a single P. falciparum–infected blood meal via membrane and maintained on 10% sucrose subsequently. (D) Fecundity: Blue squares represent number of eggs laid by a single female (that received RNAi treatment against the given genes) after a single blood meal; the red horizontal bars represent the median number of eggs laid per female, and black bars represent the 95% confidence interval. Data was subject to Mann-Whitney statistical tests, and plots include data from three independent biological replicates. Hatch rates indicate the average percentage of eggs giving rise to 2nd/3rd instar larvae as determined by three biological replicates. Standard deviations derived from these replicates are given as ±. P.f., P. falciparum; Non-inj, non-injected.
How the Toll and Imd immune signaling pathways mediate anti-bacterial and anti-Plasmodium responses through the Rel1 and Rel2 transcription factors is of key interest, but only recently have some details about pathway regulation become known. Several recent discoveries have shed light on the mechanisms by which pathogens trigger immune gene transcription via Relish/Rel2. Kim and colleagues have shown in Drosophila that Caspar is likely to inhibit Dredd-dependent cleavage of Relish . However, in both mosquitoes and mosquito cell lines, Rel2 has been shown to have two active isoforms, one long and one short, with differences in their gene targets ,. Considering that only the long form, Rel2-F, has inhibitory domains that need to be cleaved for activation, Caspar may only be regulating one branch of Rel2-dependent transcription. Rel2-F has also been shown to be involved in regulating transcription of key Imd pathway marker genes and melanization, and in reducing the number of P. berghei parasites in the midgut ,; however, because our dsRNAs target common domains of both Rel2 forms, we cannot rule out the possibility that Caspar may also be somehow regulating Rel2-S in the mosquito.
The mosquito's immune response against Plasmodium is currently under scrutiny as a target for malaria control strategies yet there is much to learn about how immune responses are mounted against Plasmodium and what the physiological implications are or how the responses are conserved.
Our data first indicate that manipulation of the mosquito's immune system can produce a near-complete loss of the vector's ability to transmit an unusually virulent strain of the human malaria parasite. Note that we used a P. falciparum strain that produces exceptionally high infection levels when compared to naturally acquired Plasmodium in the field . This exceptionally virulent strain failed to develop in 85% of the Caspar-depleted mosquitoes, and even those mosquitoes that became infected showed a 94% loss of oocysts when compared to the controls (Figure 2A). Caspar-depleted A. gambiae are therefore likely to be completely refractory to natural parasites in the field.
Second, we establish that the reduction in oocysts resulting from depletion of either Cactus or Caspar indicates that both the Toll and Imd immune pathways are involved in the defense against both P. falciparum and P. berghei, but to different degrees depending on the parasite species (Figure 2A and 2B). This and other studies have shown that activation of the Toll pathway through cactus silencing renders mosquitoes almost non-permissive to infection with the rodent malaria-causing parasite P. berghei , while our data indicate that the same treatment results in an increased but only partial resistance to infection with the human P. falciparum. Previous studies have also shown profound differences in the immune responses mounted by A. gambiae to P. berghei and P. falciparum ,. Our data further support the existence of a distinction between immunity-based resistance to rodent and human malaria parasites and this distinction appears to depend, at least in part, on which Rel factor is activated; i.e. Rel2-based immunity seems most efficient against P. falciparum while Rel1-based immunity is most efficient against P. berghei. It will be interesting to identify the underlying cause of this distinction; experiments that identify mosquito proteins specifically regulated by either parasite coupled with experiments identifying unique parasite surface molecules may help clarify the distinction.
Third, we observe that the infection-resistant phenotype is not constrained by Anopheles species; silencing A. albimanus and A. stephensi caspar orthologs reproduces the reduction in P. falciparum oocysts (Figure 2C and 2D). This, in light of the relative divergence of these mosquito species, brings about important insight into both the evolution of the Anopheles-Plasmodium interaction as well as the implications for the development of malaria control strategies based on mosquito immunity. Co-evolution is at the crux of the complex interactions between vector, parasite and host. How is it that some interactions can be consistent from one species to another while others are unique? What pressures are exerted by the environment or microbial exposures that precipitate changes or, alternatively, what needs are only met through conservation? Caspar's proposed role in the Imd pathway obviously marks a position in the immune system that is needed by mosquitoes to combat P. falciparum and, as a negative regulator of a powerful pathway, may be involved in maintaining the evolutionary balance between controlling the parasite and avoiding chronic immune up-regulation. But how, then, does Caspar depletion circumvent species-specificity? At the cellular and molecular level, the possible differences between species in the Anopheles genera are indefinite, meaning slight alterations in any number of molecules, cells or mechanisms could be responsible for variable success of an anti-Plasmodium response. We think it is likely that Caspar depletion transcends this limitation because we have targeted a conserved protein in a conserved pathway that leads to the activation of a battery of anti-Plasmodium mechanisms. It is certainly possible that some constituents of these downstream mechanisms differ from mosquito species to species but the sum of all parts is a robust overall anti-Plasmodium falciparum immune response. This same principle would mean that it is unlikely that P. falciparum would acquire resistance to this strategy since there are multiple effectors working in concert. From a malaria control aspect, in this way we can gain refractoriness in a variety of vectors.
Fourth, we have begun to delve deeper into the molecular outcome of caspar silencing. Dissection of the downstream battery of immune effectors and how/if they interact is a formidable task and would require extensive experimentation and collaborative efforts. However, using transcriptional and functional genomics, we do establish here that such a mechanism exists and that several key anti-Plasmodium genes are involved. The microarray-derived gene expression profiles illustrate that silencing negative regulators activates an arsenal of genes, immune-relevant and otherwise, that may or may not have a direct effect on malaria parasites. Depletion of Cactus resulted in the transcriptional regulation of a more than five-fold higher number of genes than did Caspar depletion, suggesting that Rel1 is a more ubiquitous transcription factor than Rel2 (Figure 3A and 3B). In fact, the Toll pathway has been linked with a variety of processes in development and hemocyte proliferation, and this range of effects was reflected by the broad range of functional gene groups that we found to be influenced by cactus silencing (Figure 3A) ,,. Similar observations have also been made in Dif/Dorsal-deficient D. melanogaster larvae and other Toll pathway factor mutants that have shown differences in the expression of a large number of non-immune genes, whereas mutations in Imd factors have affected immune gene expression more specifically . Hence, the Toll pathway appears to be a more general and versatile signaling pathway, while Imd is more immunity-specific. Many genes that responded to Cactus depletion are involved in replication, transcription and translation—a likely consequence of the cellular response needed to accommodate the increased activation of a potent transcription factor such as Rel1 and the hemocyte proliferation known to follow Toll pathway activation. Immunity, redox/stress responses and metabolism were also well-represented; immunity and redox reflect Rel1's major role in the response to pathogens and the stress caused by infection while the concurrent enrichment of metabolism- and apoptosis-related genes may provide a transcriptional link between the immune response and recovery from infection.
Although caspar silencing influenced transcription of significantly fewer genes, a considerable proportion of regulated genes belonged to the immunity class (see further discussion on individual genes in Text S1). Within this class were genes encoding quite a few known or putative anti-Plasmodium effectors that are good candidates for mediating the molecular outcome of caspar silencing that results in parasite killing. Some of these candidates, such as FBN9, TEP1 and LRRD7 (APL2), have already been described as performing anti-Plasmodium roles and we have shown here that they display a temporally regulated transcription profile when caspar is silenced (Figure 3C) ,,. We focused on these 3 genes because of their relevance to the infection phenotype addressed in this study. Using co-silencing techniques, we found that depletion of Caspar cannot confer resistance to P. falciparum when FBN9, TEP1 or LRRD7 was co-depleted (Figure 4). These double-silenced mosquitoes harbored similar numbers of oocysts as mosquitoes depleted of the effector alone. Intriguingly, double silenced mosquitoes tended to carry fewer oocysts than the singly silenced which further our theory that a battery of anti-Plasmodium genes, and not just one or two effectors, is regulated by Caspar. This was further illustrated by cocktail silencing experiments in which Caspar, along with two or more effectors were depleted. These triple gene-silenced mosquitoes showed a slightly greater (though not additive) infection intensities compared to those with just caspar and a single effector silenced, suggesting a concerted effort occurring either downstream or in parallel to Caspar. That the Imd pathway could control regulation of a fibrinogen-domain-containing molecule and a complement-like molecule that together interact to combat invading parasites is not unlikely. In vertebrates, ficolins are the fibrinogen-like domain containing pattern recognition receptors that activate the lectin complement pathway ,. Evidence of lectin pathway components in chordates and jawless vertebrates suggests that it is the most ancient complement activation pathway ,. The precedence set in the vertebrate system for these two molecules to cooperate to destroy pathogens as well as the observation that both TEP1 and FBN9 co-localize to the parasite surface justify speculation that a lectin complement pathway–like mechanism may also exist in mosquitoes ( and Dimopoulos lab, submitted).
Finally, to investigate the potential fitness impact of this highly potent anti-Plasmodium defense, we performed several proof-of-principle assays to determine if longevity or fecundity could be influenced by the RNAi-mediated transient immune response activation. We concede that this is by no means a thorough study of how Imd and Toll activation pathway activation impact fitness, but it provides baseline indications on any obvious physiological consequences of this immune boosting. The fact that caspar-silenced, but not cactus-silenced, mosquitoes lived as long as controls indicates that the products of the Imd, but not the Toll, pathway have a negligible effect on longevity under these conditions. Since our gene expression data indicated that cactus silencing influences five times more genes than does caspar silencing, it may be that the Toll pathway's transcriptional output is more costly than that of the more immune-specific Imd pathway. This difference could also reflect a greater toxicity of Toll products in the host. Reduced fecundity could also impart a reduction in fitness yet we observed that the same number of viable offspring were produced per caspar-silenced female as dsGFP-treated or non-injected controls; taken with the longevity data, we conclude that fitness by these measures and in this environment is unimpaired by the transient Rel2 –mediated immune response. The contrasting fitness cost of cactus-silencing suggests that manipulation of the Toll pathway may be too detrimental to mosquito fitness for its use in a malaria control strategy, though it would be quite interesting to continue investigating how Toll pathway activation impacts fitness and how insects negotiate the cost/benefit of Toll pathway activity. On the other hand, that Caspar manipulation does not confer a noticeable fitness cost warrants future evaluation in more realistic contexts and further analysis of its molecular mechanism. We do suspect that fitness costs will be less obvious in this context than in others, since the immune induction here was not sustained for a lifetime but was relatively temporary because of the kinetics of the RNAi process. This situation is in accordance with reports showing that sustained NF-kappaB-dependent chronic immune responses are correlated with a shorter life while temporary acute responses are not . We also questioned whether this analysis could have become compromised by the experimental method that required injection of dsRNA which also could facilitate introduction of bacteria that could alter survivorship; the caspar dsRNA treated mosquitoes may in this case experience an advantage due to immune activation We must use this technique as gene silencing and over expression by other methods are prohibitively difficult in A. gambiae. As a control, hemolymph from mosquitoes injected with dsRNA against caspar and GFP as well as unwounded mosquitoes was perfused with saline and plated on LB agar at sterile conditions. Resulting colony counts indicated that individual mosquitoes from all groups contained a large range of bacterial quantities and no significant differences were found among groups suggesting that if bacteria are introduced into the hemocoel during injection, they are in negligible amounts or are unable to survive and/or proliferate (data not shown).
Upon caspar silencing, we did not observe any spontaneous melanization that was the compelling phenotype for the discovery of Caspar deficiency in Drosophila . It is likely that the absence of melanization in mosquitoes simply reflects differences in how deficiencies are generated; a P-element insertion in Drosophila can cause Caspar loss of function throughout the body for a lifetime while the RNAi-mediated silencing strategy we employed is transient and causes differing levels of transcript degradation in different tissues. Because of this, we can not rule out that a constitutive and thorough Caspar loss of function would cause a similar hyper-melanization phenotype in mosquitoes.
By manipulating Caspar and Cactus in the present study, we were able to produce a transcriptional immune response that potentially involved a variety of anti-Plasmodium factors. Thus, caspar silencing was probably so effective against P. falciparum because it simultaneously enhanced an entire battery of relevant effectors and mechanisms. Global induction is advantageous for development of control strategies, since it avoids reliance on a single gene and the associated limitations in effectiveness: that it may only be effective against a certain parasite stage or strain and that resistance may more easily develop. This may also be why, as a physiological and biochemical mechanism, immune system activation produces a more extensive reduction in parasite burden than synthetic methods. If our strategy of depleting Caspar proves to be an effective way of limiting vector competence, short-term immune induction could be achieved through infection-inducible promoters that drive recombinant Rel2 expression. A further understanding of the impact of immune pathway activation on the mosquito's fitness will necessitate not only the development of an injury-independent mechanism but also the assessment of fitness under field conditions.
Materials and Methods
Identification of A. gambiae Caspar
Peptide sequences for Drosophila Caspar (CG8400) and its predicted A. gambiae ortholog were retrieved from Ensembl and subject to alignment using BLAST and Clustal W and the BLOSUM62 scoring matrix. Sequence alignment achieved an expected value of 5e−150. Domain similarity was determined by BLAST alignment of amino acid sequences of Drosophila Caspar regions as defined by Kim et al.  against the entire Anopheles Caspar sequence. Domain regions were then verified using the SMART database version 5.1 .
A. gambiae Keele strain, A. albimanus Santa Tecla and A. stephensi mosquitoes were maintained on a 10% sugar solution at 27°C and 80% humidity with a 12-h light/dark cycle according to standard procedures . For all mosquitoes, ∼250 larvae per 30×34 cm tray were reared with daily addition of cat food pellets and a ground fish food supplement upon water change. Adults were reared in a 20×20×20 cm3 cage and provided 10% sucrose.
RNAi gene silencing
Assays were performed according to standard protocol . Sense and antisense RNAs were synthesized from ∼300–600 bp PCR-amplified gene fragments using the T7 Megascript kit (Ambion) and primers indicated in Text S1. About 69 nl dsRNA (2–3 µg/µl) in water was introduced into the thorax of cold-anesthetized 2–4 day old female mosquitoes by a nano-injector (Nanoject, Drummond) with glass capillary needles according to an established methodology .
Real-time quantitative PCR expression analysis
Assays were performed according to standard protocol . Total RNA from adult females was extracted using the RNeasy kit (QIAGEN), quantified using a Beckman DU640 spectrophotometer and subjected to reverse transcription using Superscript III (Invitrogen) with random hexamers. Real-time quantification was performed using the QuantiTect SYBR Green PCR Kit (Qiagen) and ABI Detection System ABI Prism 7000. Primer sequences are given in Text S1. All qPCR reactions were performed in triplicate; to check for the specificity of the PCR reactions, melting curves were analyzed for each data point. The levels of expression in gene-silenced samples were determined by normalizing cDNAs using the ribosomal protein S7 gene and comparing to controls treated with dsRNA against GFP. P-values were determined using a student's T-test.
Challenge with Plasmodium
P. falciparum and P. berghei infections were administered according to standard protocol . For P. falciparum infections, mosquitoes were fed on NK54 gametocytes in human blood through a membrane feeder at 37°C 4 days after dsRNA treatment. Unfed mosquitoes were removed within 24 h after feeding, and the rest were maintained at 24°C for 7 days. For P. berghei infections, mosquitoes were fed on Swiss Webster mice infected with the wt Anka 2.34 strain of P. berghei at 21°C 4 days after dsRNA treatment. Unfed mosquitoes were removed from the group within 24 h after feeding and the rest were maintained at 21°C for 14 days. For both infections, mosquito midguts were dissected and stained with mercurochrome, and oocyst numbers were recorded using a light-contrast microscope (Olympus). Each assay was done with at least 25 mosquitoes, and data represent the results of three independent assays. P-values were determined using a Mann-Whitney test.
Sequencing of A. albimanus and A. stephensi caspar and cactus
Using known sequences from A. gambiae, D. melanogaster and A. aegypti, degenerate primer pairs (with sequence bias toward A. gambiae) were designed to amplify regions spanning the entire transcript of either gene. Regions were amplified from total cDNA from each mosquito species using standard PCR protocol and cycling program. PCR products were excised from a 1% agarose gel, extracted (Qiagen Qiaquick gel extraction kit), sequenced (Applied Biosystems 3730×l DNA Analyzer), and aligned to A. gambiae sequenced using BLAST and Clustal W and the BLOSUM62 scoring matrix. Compared to A. gambiae, sequences of regions of A. albimanus cactus and caspar had identities of 77–85% and 77–100%, respectively while regions of A. stephensi cactus and caspar had identities of 70–92% and 80–93%, respectively. Regions used for generating double-stranded RNA achieved the following nucleotide identities: A. albimanus cactus, 77%; A. albimanus caspar, 79%; A. albimanus cactus 75% and A. stephensi caspar, 92%.
Assays and analysis were performed according to standard protocol . All arrays performed using female A. gambiae at 3 days post silencing. Gene expression values were compared between Cactus- and Caspar-depleted adult female mosquitoes and dsGFP-treated controls. Total RNA was extracted from 10–15 whole mosquitoes 3 days after dsRNA treatment using the RNeasy kit (QIAGEN). Quantification of RNA was performed using a Beckman DU640 spectrophotometer, and quality was assessed by RNA Nano LabChip analysis on an Agilent Bioanalyzer 2100. Probes were synthesized with 2–3 µg RNA using the Agilent Technologies low-input RNA labeling kit according to the manufacturer's instructions. Hybridizations were done with the Agilent technologies in situ hybridization kit according to manufacturer's instructions. Arrays were washed then dried using pressurized air. Microarray scanning was done with an AXON 4200AL scanner, with the laser power set to 60% and the PMT gain adjusted manually to maximize effective dynamic range and avoid spot saturation. Images were analyzed with Genepix 6.0 software to determine spot size, location and quality, and potentially confounding spots were manually removed from the analysis. The data were then processed with TIGR MIDAS software . The intensity threshold was set to 100 for both Cy5 and Cy3 channels, and the signal-to-background cutoff was set to 2.0 in both channels. Data for each experimental condition were derived from three biological replicates. The median spot intensities for each spot meeting the above criteria were normalized according to a LOWESS normalization method. The TIGR MeV software  was then used to Log2 transform the Cy5/Cy3 ratios and perform t-tests with the following parameters: mean value to be tested against = 0, the Welsh approximation method for degree of freedom calculation, P-values based on t-distribution, the overall alpha (critical p-value) set to 0.05, no p-value correction. According to established methods, a cut-off value for the significance of the gene regulation was set to 0.8 in a log2 scale (1.74-fold ratio) . Values for genes that had a significant p-value for one experimental set were included in other experimental sets, providing that the direction of regulation was consistent and the value was within a range of <0.5 fold.
Two-day-old adult female A. gambiae were treated with dsRNA against cactus, caspar or GFP as described, then incubated at 27°C with 70% humidity while being maintained on sterilized 10% sucrose solution. Injected mosquitoes and non-injected mosquitoes from the same generation were monitored simultaneously to control for injection-induced mortality. All cohorts were monitored daily for survival, and dead mosquitoes were removed each day. Monitoring continued until all mosquitoes had perished. Percentages represent the mean survival between 3 biological replicates of 50 mosquitoes each. Statistical significance was determined using Kaplan-Meier and log-rank analyses.
For each of three biological replicates, at least 30 two-day-old female mosquitoes were treated with dsRNA then at 3 d.p.i. (days post injection) allowed to feed on human blood through an artificial membrane system for 30 minutes. Fed mosquitoes were transferred to individual wax-lined cardboard cups outfitted with cotton soaked in 10% sucrose solution and an oviposition cup filled with water and lined with filter paper. Individual chambers were incubated under normal rearing conditions. Eggs oviposited on filter paper were counted after 2 days using light microscopy. Those females with no eggs on day 2 were maintained and filter papers were examined on day 3. After each count, eggs were submerged en masse in a standard larval pan for rearing according to standard methods (see rearing methods). Second or third instar larvae were counted and removed from larval pan daily. Statistical significance of oviposition was determined using Mann-Whitney and statistical significance of hatch rates was determined using one way ANOVA (analysis of variance).
Hemolymph perfusion and bacterial colony counts
For each of three biological replicates, at least 10 two-day old female mosquitoes were microinjected with dsRNA or reserved as non-injected controls. Three days post silencing, mosquitoes were surface sterilized with 70% ethnol and PBS and sterile PBS was perfused through the thorax and collected with a sterile needle according to previous established protocol (ref). Collected hemolymph was serially diluted in PBS and dilutions were each plated on LB agar. Plates were sealed and kept in insectary conditions for 2 days then colonies were counted. Number of bacteria per mosquito was determined using an average of all serial dilutions for that individual.
All animals were handled in strict accordance with good animal practice as defined by the relevant national and/or local animal welfare bodies, and all animal work was approved by the appropriate committee.
Validation of gene expression analyses of cactus- and caspar-silenced mosquitoes. (A,B) Validation of microarray using qRT-PCR. Array-derived gene expression values are plotted on the x-axis while averages of three real-time PCR-derived gene expression values from biological replicates are plotted on the y-axis. Each point represents the log-transformed values for one tested gene; which are given in Tables S1A and S1B. Line of best fit (Microsoft Excel) is included. (A) Gene expression following cactus silencing (compared to GFP). The best-fit linear-regression analysis (R2 = 0.770), and the slope of the regression line (m = 1.15) demonstrated a high degree of correlation between gene expression magnitudes determined via array and real-time assays. (B) Gene expression following caspar silencing (compared to GFP). The best-fit linear-regression analysis (R2 = 0.772) and the slope of the regression line (m = .64) demonstrated a reasonably high degree of correlation between gene expression magnitudes determined via array and real-time assays.
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Gene expression in cactus-, caspar-, cactus/rel1- and caspar/rel2-silenced mosquitoes.
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Immune genes regulated by negative regulator silencing.
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Cactus gene-silenced transcriptome expressed as log2 transformed cactus gene-silenced/GFP dsRNA expression ratio.
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Caspar gene-silenced transcriptome expressed as log2 transformed caspar gene-silenced/GFP dsRNA expression ratio.
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We are grateful to the MR4 for provision of A. albimanus eggs and to Dr. Zhiyong Xi for assistance with the microarray data analyses. We thank the microarray core facility, the parasitology core facility, animal care facility, and the insectary personnel at the Johns Hopkins Malaria Research Institute for assistance with microarray analyses, P. falciparum culture, mouse care, and mosquito rearing.
Conceived and designed the experiments: LSG GD. Performed the experiments: LSG YD. Analyzed the data: LSG YD GD. Wrote the paper: LSG GD.
- 1. Meister S, Koutsos AC, Christophides GK (2004) The Plasmodium parasite—a ‘new’ challenge for insect innate immunity. Int J Parasitol 34: 1473–82.
- 2. Michel K, Kafatos FC (2005) Mosquito immunity against Plasmodium. Ins Biochem Mol Biol 35: 677–689.
- 3. Christophides GK, Zdobnov E, Barillas-Mury C, Birney E, Blandin S, et al. (2002) Immunity-related genes and gene-families in Anopheles gambiae. Science 298: 159–165.
- 4. Meister S, Kanzok SM, Zheng XL, Luna C, Li TR, et al. (2005) Immune signaling pathways regulating bacterial and malaria parasite infection of the mosquito Anopheles gambiae. Proc Natl Acad Sci U S A 102: 11420–11425.
- 5. 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.
- 6. Dong Y, Aguilar A, 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.
- 7. Cohuet A, Osta MA, Morlais I, Awono-Ambene PH, Michel K, et al. (2006) Anopheles and Plasmodium: from laboratory models to natural systems in the field. EMBO Rep 7: 1285–1289.
- 8. Lemaitre B, Meister M, Govind S, Georgel P, Steward R, et al. (1995) Functional analysis and regulation of nuclear import of dorsal during the immune response in Drosophila. EMBO J 14: 536–545.
- 9. Barillas-Mury C, Charlesworth A, Gross I, Richman A, Hoffmann JA, et al. (1996) Immune factor Gambif1, a new rel family member from the human malaria vector, Anopheles gambiae. EMBO J 15: 4961–4701.
- 10. Wu LP, Anderson KV (1998) Regulated nuclear import of Rel proteins in the Drosophila immune response. Nature 392: 93–97.
- 11. Rutschmann S, Jung AC, Hetru C, Reichhart JM, Hoffmann JA, et al. (2000) The Rel protein Dif mediates the antifungal but not the antibacterial host defense in Drosophila. Immunity 12: 569–580.
- 12. Belvin MP, Anderson KV (1996) A conserved signaling pathway: the Drosophila toll-dorsal pathway. Annu Rev Cell Dev Biol 12: 393–416.
- 13. Belvin MP, Jin Y, Anderson KV (1995) Cactus protein degration mediates Drosophila dorsal-ventral signaling. Genes Dev 9: 783–793.
- 14. Stoven S, Ando I, Kadalayil L, Engstrom Y, Hultmark D (2000) Activation of Drosophila NF-kappaB factor Relish by rapid proteolytic cleavage. EMBO Rep 1: 347–152.
- 15. Stoven S, Silverman N, Junell A, Hedengren-Olcott M, Erturk D, et al. (2003) Caspase-mediated processing of the Drosophila NF-kappaB factor Relish. Proc Natl Acad Sci USA 100: 5991–5996.
- 16. Kim M, Lee JH, Lee SY, Kim E, Chung J (2006) Caspar, a suppressor of antibacterial immunity in Drosophila. Proc Natl Acad Sci U S A 103: 16358–16363.
- 17. Dimopoulos G, Seeley D, Wolf A, Kafatos FC (1998) Malaria infection of the mosquito Anopheles gambiae activates immune-responsive genes during critical transition stages of the parasite life cycle. EMBO J 17: 6115–6123.
- 18. Dimopoulos G, Christophides GK, Meister S, Schultz J, White KP, et al. (2002) Genome expression analysis of Anopheles gambiae: responses to injury, bacterial challenge, and malaria infection. Proc Natl Acad Sci U S A 99: 8814–8819.
- 19. Aguilar R, Jedlicka AE, Mintz M, Mahairaki V, Scott AL, et al. (2005) Global gene expression analysis of Anopheles gambiae responses to microbial challenge. Insect Biochem Mol Biol 35: 709–719.
- 20. Vlachou D, Schlegelmilch T, Christophides GK, Kafatos FC (2005) Functional genomic analysis of midgut epithelial responses in Anopheles during Plasmodium invasion. Curr Biol 15: 1185–1195.
- 21. 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.
- 22. Osta MA, Christophides GK, Kafatos FC (2004) Effects of mosquito genes on Plasmodium development. Science 303: 2030–2032.
- 23. Parmakelis A, Slotman MA, Marshall JC, Awono-Ambene PH, Antonio-Nkondjio C, et al. (2008) The molecular evolution of four anti-malarial immune genes in the Anopheles gambiae species complex. BMC Evol Biol 8: 79.
- 24. Simard F, Licht M, Besansky NJ, Lehmann T (2007) Polymorphism at the defensin gene in the Anopheles gambiae complex: testing different selection hypotheses. Infect Genet Evol 7: 285–292.
- 25. Lazzaro BP (2008) Natural selection on the Drosophila antimicrobial immune system. Curr Opin Microbiol 11: 284–289.
- 26. Sackton TB, Lazzaro BP, Schlenke TA, Evans JD, Hultmark D, et al. (2007) Dynamic evolution of the innate immune system in Drosophila. Nat Genes 39: 1461–1468.
- 27. Libert S, Chao Y, Chu X, Pletcher SD (2006) Trade-offs between longevity and pathogen resistance in Drosophila melanogaster are mediated by NFkappaB signaling. Aging. Cell 5: 533–543.
- 28. Luna C, Hoa NT, Lin H, Zhang L, Nguyen HLA, et al. (2006) Expression of immune responsive genes in cell lines from two difference Anopheline species. Ins Mol Biol 15: 721–729.
- 29. Sallum MAM, Schultz TR, Wilkerson RC (2000) Phylogeny of Anophelinae (Diptera, Culicidae) based on morphological characters. Systematics 93: 745–775.
- 30. Krzywinski J, Wilkerson RC, Besansky NJ (2001) Toward Understanding Anophelinae (Diptera, Culicidae) phylogeny: insights from nuclear single-copy genes and the weight of evidence. Syst Biol 50: 540–556.
- 31. Sallum MAM, Schultz TR, Foster PG, Aronstein K, Wirtz RA, et al. (2002) Phylogeny of Anophelinae (Diptera: Culicidae) based on nuclear ribosomal and mitochondrial DNA sequences. Systematic Entomology 27: 361 382.
- 32. Riehle MM, Markianos K, Lambrechts L, Xia A, Sharakhov J, et al. (2006) Natural malaria infection in Anopheles gambiae is regulated by a single genomic control region. Science 312: 577–579.
- 33. Robb T, Forbes M (2006) Age-dependent induction of immunity and subsequent survival costs in males and females of a temperate damselfly. BMC Ecol 6: 15.
- 34. Luna C, Wang X, Huang Y, Zhang J, Zheng L (2002) Characterization of four Toll related genes during development and immune responses in Anopheles gambiae. Ins Biochem Mol Biol 32: 1171–1179.
- 35. Pringle G (1966) A quantitative study of naturally-acquired malaria infections in Anopheles gambiae and Anopheles funestus in a highly malarious area of East Africa. Trans R Soc Trop Med Hyg 60: 626–632.
- 36. Qiu P, Pan PC, Govind S (1998) A role for the Drosophila Toll/Cactus pathway in larval hematopoiesis. Development 125: 1909–1920.
- 37. Pal S, Wu J, Wu LP (2007) Microarray analyses reveal distinct roles for Rel proteins in the Drosophila immune response. Dev Comp Immunol 32: 50–60.
- 38. Liu Y, Endo Y, Iwaki D, Nakata M, Matsushita M, et al. (2005) Human M-Ficolin Is a Secretory Protein That Activates the Lectin Complement Pathway. J Immunol 175: 3150–3156.
- 39. Matsushita M, Endo Y, Hamasaki N, Fujita T (2001) Activation of the lectin complement pathway by ficolins. Int Immunopharmacology 1: 359–363.
- 40. Matsushita M, Matsushita A, Endo Y, Nakata M, Kojima N, et al. (2004) Origin of the classical complement pathway: lamprey orthologue of mammalian C1q acts as a lectin. Proc Natl Acad Sci U S A 101: 10127–10131.
- 41. Endo T, Takahashi M, Fujita T (2006) Lectin complement system and pattern recognition. Immunobiology 211: 283–293.
- 42. Letunic I, Copley RR, Pils B, Pinkert S, Schultz J, et al. (2006) SMART5: domains in the context of genomes and networks. Nucleic Acids Res 34(Database): D257–D260.
- 43. Benedict MQ (1997) Care and maintenance of anopheline mosquitoes. In: Crampton JM, Beard CB, Louis C, editors. The molecular biology of disease vectors: A methods manual. London: Champman & Hall. pp. 3–12.
- 44. Dudoit S, Gentleman RC, Quackenbush J (2003) Open source software for the analysis of microarray data. Biotechniques (Suppl) 45–51.
- 45. Yang IV, Chen E, Hasseman JP, Liang W, Frank BC, et al. (2002) Within the fold: assessing differential expression measures and reproducibility in microarray assays. Genome Biol 3: research0062.