Hemocyte Differentiation Mediates Innate Immune Memory in Anopheles gambiae Mosquitoes

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Science  10 Sep 2010:
Vol. 329, Issue 5997, pp. 1353-1355
DOI: 10.1126/science.1190689

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Mosquito midgut invasion by ookinetes of the malaria parasite Plasmodium disrupts the barriers that normally prevent the gut microbiota from coming in direct contact with epithelial cells. This triggers a long-lived response characterized by increased abundance of granulocytes, a subpopulation of hemocytes that circulates in the insect’s hemocoel, and enhanced immunity to bacteria that indirectly reduces survival of Plasmodium parasites upon reinfection. In mosquitoes, differentiation of hemocytes was necessary and sufficient to confer innate immune memory.

The innate immune system is thought to be hard-wired and unable to establish immunological memory (1). Insects lack adaptive immunity and rely on the innate immune system to mount defense responses against pathogenic organisms; however, memory-like responses have been described in invertebrates, a phenomena that has been termed immune priming (2). There are multiple examples of nonspecific (35) and pathogen-specific (611) priming in insects that can be long-lasting. Although these studies challenge the dogma that invertebrates are incapable of adaptive immune responses, a mechanism for innate immune memory has not been established.

Anopheles gambiae mosquitoes are the major vectors of Plasmodium falciparum malaria in Africa. In the present study, we found that Plasmodium ookinete invasion of the mosquito midgut in the presence of gut bacteria primed a robust long-lived enhanced antibacterial response that also reduced Plasmodium survival upon rechallenge. Immune priming resulted in quantitative and qualitative differentiation of hemocytes, the insect equivalent of white blood cells, that persisted for the lifespan of the mosquito.

We investigated the effect of preexposure of mosquitoes to Plasmodium infection on a subsequent infection (fig. S1) (12). Two groups of mosquitoes were fed on the same infected mouse. One group was placed at 28°C immediately after blood feeding, a temperature that prevents Plasmodium berghei ookinete formation and mosquito infection (fig. S2). We refer to these mosquitoes as the naïve group. The challenged group was kept at 21°C for 48 hours to allow ookinete formation and midgut invasion and was then switched to 28°C to reduce oocyst survival (fig. S2). Seven days postfeeding (dpf), both groups were infected by feeding on a second mouse. Reexposure to Plasmodium infection greatly reduced the intensity of infection in the challenged group (Fig. 1A) (P < 0.005). This immune enhancement was also observed in females rechallenged 14 days postpriming (dpp) (P < 0.0005) (Fig. 1B). The time between priming and rechallenge was not extended because of age-related mosquito mortality. Preexposure of mosquito females to P. falciparum (NF54 strain) infection had a similar effect, reducing oocyst density when rechallenged with the same parasite (P < 0.05, Mann-Whitney test) (Fig. 1C and fig. S3).

Fig. 1

Effect of preexposure to Plasmodium infection on the immune response to subsequent infections. (A) 7 dpp and (B) 14 dpp with P. berghei in naïve (Nv) or challenged (Ch) mosquitoes. (C) Effect of prechallenge with P. falciparum on a second infection at 7 dpp. Plasmodium infections were evaluated 7 days after the second infection. Effect of eliminating the gut microbiota with oral antibiotics before the (D) first and (E) second challenge with P. berghei on a second infection 7 dpp. Each circle represents the number of parasites in an individual midgut, and lines indicate the medians.

Large numbers of commensal bacteria are present in the midgut lumen when Plasmodium ookinetes invade epithelial cells. The blood meal is surrounded by a chitinous peritrophic matrix (PM) that normally prevents bacteria from interacting directly with epithelial cells, but ookinetes disrupt this barrier (13) to invade midgut cells (fig. S4), causing irreversible damage (14). The PM sac containing the blood-meal remnants is expelled when digestion is completed, and a new PM sac forms with each subsequent feeding. Elimination of the gut microbiota enhances Plasmodium infection (1517), and activation of some mosquito antibacterial responses have been shown to indirectly kill Plasmodium (17).

Gut bacteria were eliminated by oral administration of antibiotics before the first feeding (fig. S1, yellow area), which prevented immune priming to Plasmodium (Fig. 1D). Then priming was allowed to occur in the presence of bacteria, but antibiotics were given 2 days before the second infection (fig. S1, beige area). Elimination of the gut microbiota when mosquitoes are rechallenged prevented elicitation of the priming response (Fig. 1E). It was the interaction between bacteria and invaded midgut cells that appeared to elicit the response, which indicates that the decrease in Plasmodium infection in the challenged group (Fig. 1, A and B) was not due to persistent immune activation in response to the first plasmodial infection.

The effect of priming on mosquito commensal bacteria was investigated. Total bacteria in challenged mosquitoes 7 dpp were 1% of the amount in naïve mosquitos (P < 0.005) (Fig. 2A). Bacterial levels in the midgut were similar between naïve and challenged groups before the second feeding (Fig. 2B, gray). Bacteria proliferated when either naïve or challenged mosquitoes received a second meal, but bacterial levels were significantly reduced in the challenged group (P < 0.001) 24 hours postinfection (hpi) (Fig. 2B, blue).

Fig. 2

Effect of immune priming with Plasmodium or bacteria on commensal bacteria, hemocyte populations, and gut-associated hemocyte-specific antiplasmodial mRNAs. (A) Effect of priming on whole-body bacterial levels in naïve (Nv) and challenged (Ch) mosquitoes 7 dpp. Bars represent mean ± SEM; asterisks indicate differences that are statistically significant (unpaired two-tailed t test). (B) Total midgut bacteria before (Be) or 24 hours after (Af) a second infectious meal was given 7 dpp. Bacterial 16S ribosomal RNA (rRNA) levels were determined by using real-time polymerase chain reaction (PCR). Effect of immune priming on the relative abundance of (C) granulocytes and (D) prohemocytes 7 dpp in the presence or absence of gut microbiota. Effect of immune priming on the relative abundance of TEP1 and LRIM1 mRNAs associated with the midgut or circulating hemocytes in (E) the presence or (F) the absence of gut microbiota determined before (gray) or 24 hours after (red) a second infectious meal was given 7 dpp.

No significant difference in total number of hemocytes or in relative abundance of oenocytoids (fig. S5) was observed between naïve and challenged mosquitoes 7 dpp; however, the granulocyte population increased by up to 3.2-fold (Fig. 2C) (P < 0.01), and prohemocytes decreased by 10% (Fig. 2D) (P < 0.05) in the challenged group, suggesting that prohemocyte precursors differentiated into granulocytes. This response was still present 14 dpp (fig. S6) but was no longer observed when priming was prevented by eliminating the gut microbiota (Fig. 2, C and D). Hemocytes respond to ookinete invasion by attaching to the basal surface of the midgut, which increases the mRNA levels of hemocyte-specific genes such as thioester-containing protein 1 (TEP1) and leucine-rich repeat immune protein 1 (LRIM1) associated with midguts dissected 24 hpi (18, 19). This response is transient, because higher transcript levels were not detected 48 hpi (19). In our experiments, midgut invasion increased TEP1 and LRIM1 mRNA levels in naïve and challenged mosquitoes 24 hpi (Fig. 2E), but in challenged mosquitoes the increases in TEP1 and LRIM1 levels were up to 12- and 8-fold higher, respectively (P < 0.005) (Fig. 2E). As expected, a concomitant reduction in TEP1 and LRIM1 levels was observed in the population of circulating hemocytes from the same mosquitoes (P < 0.05) (Fig. 2E), which we speculate indicates that some hemocytes that express TEP1 and LRIM1 disappear from circulation as they attach to the midgut. This response was only observed when primed mosquitoes were reinfected, indicating an enhanced response to rechallenge rather than a persistent long-lasting re sponse after the initial exposure to Plasmodium and bacteria. This enhanced hemocyte response was not observed in mosquitoes in which priming was prevented by eliminating bacteria from the gut microbiota (Fig. 2F).

Morphologic differences between granulocytes from naïve and challenged mosquitoes were apparent immediately after hemocytes were placed in plastic Neubauer chambers for counting. The cytoplasm of granulocytes from challenged mosquitoes was larger and more granular, and pseudopodial extensions were observed (Fig. 3A). However, when naïve or challenged granulocytes attached to a glass surface, these morphological differences were no longer apparent (Fig. 3B). Comparison of the lectin-binding properties of naïve and challenged hemocytes to fluorescence-conjugated lectins revealed that wheat germ agglutinin (WGA) stained all hemocytes from naïve and challenged mosquitoes, including granulocytes (Fig. 3B). In contrast, only granulocytes from challenged mosquitoes were stained with Lens culinaris agglutinin (LCA) (Fig. 3B and table S1), whereas most (96%) of naïve granulocytes were negative and 4% were stained weakly (P < 0.0001; χ2).

Fig. 3

Effects of immune priming on granulocyte morphology and binding properties and of water injection on or hemolymph transfer on hemocyte populations and Plasmodium infection. (A) Morphology of naïve (Nv) and challenged (Ch) granulocytes in a plastic Neubauer chamber (scale bars indicate 7.5 μm). (B) Effect of priming on lectin-binding properties of granulocytes. Scale bars, 5 μm. (C) Effect of water injection (69 nl) on circulating granulocytes and prohemocytes. (D) Effect of water injection 7 dpp on Plasmodium infection. Effect of cell-free hemolymph transfer from Nv or Ch mosquito on (E) circulating granulocytes, oenocytoids, and prohemocytes and (F) on Plasmodium infection 4 days posttransfer. Each circle represents the number of parasites in an individual midgut, and the line indicates the median. Bars in (C) and (E) represent mean ± SEM.

We disrupted granulocytes by injecting Sephadex beads resuspended in water or phosphate-buffered saline (PBS) into the hemocoel to test whether they were necessary to elicit the priming response. A control group was injected with water alone. Unexpectedly, when challenged mosquitoes were injected with a small volume of water (69 nl), the proportion of circulating granulocytes decreased to levels similar to those of naïve mosquitoes, and differences in the proportion of prohemocytes between naïve and challenged mosquitoes were no longer observed (Fig. 3C). This one-half reduction in circulating granulocytes in the challenged group is highly significant (P < 0.0001) and abolished priming, suggesting that these cells are necessary to elicit the priming response (Fig. 3D). Priming is also disrupted when challenged mosquitoes are subjected to aseptic injury or are injected with PBS or Sephadex beads in water (fig. S7). We speculate that primed granulocytes are probably recruited to the injury site, disappear from circulation, and are no longer available to mediate an enhanced immune response when mosquitoes are reinfected with Plasmodium.

Lastly, we explored whether transfer of cell-free hemolymph or hemolymph containing hemocytes from challenged mosquitoes could confer enhanced immunity in recipient mosquitoes that had only fed on sugar. Transfer of cell-free hemolymph from challenged mosquitoes by systemic injection increased the relative abundance of circulating granulocytes and oenocytoids (Fig. 3E), decreased prohemocytes (Fig. 3E), and greatly reduced both the intensity (Fig. 3F) (P < 0.0001) and the prevalence of Plasmodium infection (from 92% to 51%; P < 0.001; χ2) in the recipients relative to mosquitoes that received hemolymph from naïve donors. When hemolymph containing hemocytes from challenged mosquitoes was transferred, granulocytes increased and prohemocytes were reduced in the recipients, but oenocytoids were not affected, and Plasmodium infection was also reduced significantly (P < 0.0001) (fig. S8). Transfer of cell-free hemolymph did not affect the total number of hemocytes in the recipients, but a significant reduction in circulating hemocytes (P < 0.005) was observed in mosquitoes that received challenged hemocytes (fig. S9). Transfer of these cells may reduce viability, proliferation, and/or adherence of endogenous hemocytes.

A strong priming response was established when ookinetes breached the gut barriers and bacteria came in contact with injured epithelial cells. The mosquito immune system was stimulated to a systemic state of enhanced immune surveillance. Upon reexposure to a similar insult, mosquitoes mounted a more effective antibacterial response that indirectly harmed Plasmodium parasites. We conclude that the mosquito immune system can adapt by modulating the abundance and responsiveness of different hemocyte populations. Exposure to Plasmodium or bacteria infection increases the proportion of circulating granulocytes and triggers changes in the morphology and binding properties of these cells. Circulating granulocytes mediate responses that enhance antiplasmodial immunity in challenged mosquitoes. Possibly, a soluble hemocyte differentiation factor(s) is released into the hemolymph of challenged mosquitoes that, when transferred, induces hemocyte differentiation in the recipients and confers enhanced antiplasmodial immunity. We propose that insect innate immune memory be defined as long-term functional changes in the immune system that allow an insect to mount a more effective immune response upon reencountering a microbe (or similar microbes). Future studies will be required to define the characteristics of this type of response and to establish how it differs from immune memory in vertebrates. Understanding the molecular mechanism(s) mediating insect immune responses such as induced hemocyte differentiation may also provide insights into the evolution of immune memory.

Supporting Online Material

Materials and Methods

Figs. S1 to S8

Table S1

References and Notes

  1. Materials and methods are available as supporting material on Science Online.
  2. This work was supported by the Intramural Research Program of the Division of Intramural Research, National Institute of Allergy and Infectious Diseases, NIH. We thank A. Laughinghouse and K. Lee for insectary support; C. Ortega for experimental support; L. Koo for confocal assistance; J. Ribeiro and J. Valenzuela for their comments and insight; and B. R. Marshall for editorial assistance. F.A.B. and L.C.A. were funded by the Conselho Nacionale de Desenvolvimento Científico e Tecnológico and Coordenação de Aperfeiçoamento de Pessoal de Nivel Superior Brazilian government agencies, respectively.
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