Original Research ARTICLE
Asaia Activates Immune Genes in Mosquito Eliciting an Anti-Plasmodium Response: Implications in Malaria Control
- School of Biosciences & Veterinary Medicine, University of Camerino, Camerino, Italy
In mosquitoes, the discovery of the numerous interactions between components of the microbiota and the host immune response opens up the attractive possibility of the development of novel control strategies against mosquito borne diseases. We have focused our attention to Asaia, a symbiont of several mosquito vectors who has been proposed as one of the most potential tool for paratransgenic applications; although being extensively characterized, its interactions with the mosquito immune system has never been investigated. Here we report a study aimed at describing the interactions between Asaia and the immune system of two vectors of malaria, Anophelesstephensi and An. gambiae. The introduction of Asaia isolates induced the activation of the basal level of mosquito immunity and lower the development of malaria parasite in An. stephensi. These findings confirm and expand the potential of Asaia in mosquito borne diseases control, not only through paratransgenesis, but also as a natural effector for mosquito immune priming.
Malaria is a mosquito-borne disease (MBD) caused by a parasite of the genus Plasmodium, responsible of about five hundred thousand deaths per year (World Health Organization, 2018). Considering the lack of an effective vaccine, chemical insecticides, applied either as Indoor Residual Spraying (IRSs) or Insecticide Treated Nets (ITNs), are the main prevention tools currently adopted (World Health Organization, 2014). Nevertheless, these preventive methods are losing their effectiveness due to onset of resistance phenomena in vector populations. Moreover, their massive use is highly toxic to both humans and the environment. During the last decades, new strategies have been developed to tackle malaria and more generally MBD’s. In particular, some studies have converged into the development of strategies known as Symbiotic Control (SC), using the symbiotic microorganisms colonizing vector hosts to combat the development of the parasite within them or to interfere with their competence and fitness (Ricci et al., 2012).
In mosquitoes, the malaria parasite completes its life-cycle starting from the ingestion of thousand gametocytes during the infected blood meal. Although thousands of gametocytes are ingested, only a small portion (about 10%) develops into ookinetes, and of these about 5% crosses the midgut epithelium to form the oocysts (Wang and Jacobs-Lorena, 2013). Nevertheless, an amplification of the parasites number occurs when the oocysts form and release thousands of sporozoites in the hemocoel that invade the salivary glands and will be injected in a next individual through the mosquito bite. The replication bottleneck occurring in the midgut is mainly due to two different mechanisms of mosquito innate immune system: (i) a humoral response involving a complement-like system and the transcriptional up-regulation of antimicrobial peptides (AMPs) and other immune effectors and (ii) a cell-mediated response, included phagocytosis and/or melanization (Clayton et al., 2014). The drastic reduction in numbers of the parasite makes this compartment, an ideal target to interfere with Plasmodium development in the mosquito.
Moreover, the direct interactions between gut microbiota and malaria parasite have been largely documented (Dong et al., 2009). In fact, bacteria can inhibit Plasmodium development producing a physical barrier that hinders the interaction between ookinetes and the midgut epithelium, or through the production of enzymes and toxins (Azambuja et al., 2005). Alternatively, components of the mosquito microbiota can indirectly cause alterations of the insect physiology inducing the activation of innate immune responses that are cross-reactive between bacteria and parasites, and adversely affect pathogen infection (Dong et al., 2009). In addition, the natural microbiota was proved to be involved in the inhibition of other pathogenic organisms in different mosquito species: bacteria of Aedes aegypti are able to induce basal-level immunity inhibiting dengue virus infection (Xi et al., 2008) and antibiotic-treated Culex bitaeniorhynchus showed higher susceptibility to the Japanese encephalitis virus (Mourya and Soman, 1985).
In light of these considerations, the objective of this study was the investigation of the immune response in Anopheles stephensi and An. gambiae mosquitoes challenged with Asaia sp.
Asaia is a symbiont of several mosquito species and it has characterized as a potential candidate for SC interventions, like paratransgensis. The features of this bacteria supporting its use in vector control applications are: i) a strict and conserved association with the mosquito host; ii) vertical and horizontal transmission routes; iii) easy cultivability and genetic transformability with exogenous DNA (Favia et al., 2007; Damiani et al., 2008; Damiani et al., 2010). Moreover, a strain of Asaia isolated from An. stephensi, has been transformed to express and secrete anti-Plasmodium molecules able to interference activity against Plasmodium berghei resulting in a significant reduction of oocysts development (Bongio and Lampe, 2015; Shane et al., 2018). Although Asaia has been characterized as a potential tool for its applications, its interactions with the mosquito immune system has never been investigated. This study aims at defining the role of this symbiont on the modulation of gene expression of mosquito immunity effectors and its effect on the progression of P. berghei infection within two of the main malaria vectors in Asia and Africa.
Materials and Methods
An. stephensi (Liston strain) and An. gambiae (G3 strain) were reared at standard laboratory conditions, at 29°C and 85% ± 5 relative humidity with photoperiods (12:12 Light–dark). Unless otherwise specified, adult insects were maintained with 5% sucrose solution ad libitum, and adult females were fed on mouse blood for egg laying. Larvae were maintained in spring water and fed daily with commercial fish food.
The Asaia SF2.1 strain isolated from An. stephensi (Favia et al., 2007) was used for mosquito colonization. Bacteria were grown 24 h at 30°C in GLY medium (25 g/L glycerol, 10 g/L yeast extract, pH 5). Two different concentrations were prepared from an overnight culture: (i) 108 cells/ml and (ii) 104 cells/ml. Dilutions were washed three times with 1 vol of 0.9% NaCl solution, centrifuged at 4,300 rpm for 10 min and then, re-suspended in 1 vol of 5% (wt/vol) sterile sucrose solution. The concentration of the cell suspensions was validated prior mosquito colonization by plating scalar dilutions on Gly agar medium (25 g/L glycerol, 10 g/L yeast extract, 20 g/L agar, pH 5) and by calculating CFU/ml.
Plasmodium berghei Infection
PbGFPCON, a GFP-tagged recombinant strain that constitutively expresses GFP at higher levels throughout the complete life cycle from an integrated transgene, was used for mosquito challenges (Franke-Fayard et al., 2004). Infected blood meals were performed using mice showing a parasitemia around 3–5% (Sinden, 1997) in a chamber at 20°C and 95± 5% humidity, a step strongly required for parasite development in laboratory conditions (Capone et al., 2013). Briefly, 8-week-old female mice were infected with P. berghei PbGFPCON by acyclic passages through an intraperitoneal injection of blood from the tail vein of an infected mouse with around 3–5% parasitemia. Infected mice were monitored every couple of days for parasitemia by fluorescent microscopy as well as gametocytemia evaluation by through Giemsa-stained blood smear.
Three groups were set up with 250 female pupae each. After emerging, mosquitoes were fed with three different diets: sterile sugar solution, sugar solution supplemented with 104 cells/ml of Asaia, and sugar solution with 108 cells/ml of Asaia. The three mosquito cohorts fed on different diets were named Sugar, Asa4, and Asa8, respectively (Figure 1). The analysis of immune genes expression and Asaia density were conducted on 12 mosquitoes for each treatment at different time-points: 1, 3, and 7 days post-emergence. At day 7, 70 mosquitoes from each group were split into three further groups: uninfected blood meal, Plasmodium-infected blood meal, and a control with constant sugar supply. Only fully engorged females were considered for further analyses. At day 8, 10 and 12 post-emergence, 9 mosquitoes from each group were sampled for further analyses.
Figure 1 Schematic representation of the experimental design. Three groups of mosquitoes were fed from the emergence for 7 days with different diets: Sugar 5%, Sugar 5% + Asaia 104 cells/ml and Sugar 5% + Asaia 108 cells/ml. At day 7 (represented by a red asterisk), 70 mosquitoes were split in three further cages and, at the same day, three different treatments were administrated: uninfected blood meal (pink), infected blood meal (green) and sugar diet (cyan). In each time-points, Asaia density and the expression level of CEC1, DEF1, CTL4 and TEP1 genes were evaluated. Moreover, Plasmodium load was assessed in mosquitoes infected with P. berghei at time-point 8, 10 and 12. The asterisk indicates the day of blood meal.
Two experimental replicates were performed and the results shown represent the average of both experiments. The experimental design and groups set-up is summarised in Figure 1.
The establishment of an Asaia-aposymbiotic population was prevented by the significantly reduced life span of antibiotic treated mosquitoes.
RNA Extraction and cDNA Synthesis.
Total RNA was extracted from single mosquitoes using RNAzol reagent (Sigma-Aldrich USA), according to the manufacturer’s instructions. cDNA was generated by reverse transcription of 1µg of total RNA using PrimeScript RT Reagent Kit (Takara, USA).
Expression of anti-microbial peptide cecropin (CEC1) and defensin (DEF1), C-type lectin 4 (CTL4) and Thioester-containing protein 1 (TEP1) was assessed in all mosquito cohorts. Moreover, Asaia density was evaluated for every group, whilst Plasmodium loads for infected mosquitoes at three different time points. The PCRs reaction included 1X SybrGreen Master Mix (Fermentas, Lithuania), 200 nM of oligonucleotides and 2µl of cDNA. Oligonucleotide sequences and their efficiency are summarized in Table S1. The efficiency of each primer set was calculated by the amplification of eight serial dilutions of cDNA.
Reactions were run on a CFX thermocycler (Bio-Rad, USA) using the following cycling conditions: 1 cycle of 95°C for 10 min, 40 -cycles of 95°C for 1 min, 60°C for 1 min, and 74°C for 30 s, with the exception of the Plasmodium-specific set whose annealing temperature was 58°C as described before (Jaramillo-Gutierrez et al., 2009).
Gene expression levels of target genes were normalized against the internal species-specific reference ribosomal gene RpS7 for An. stephensi and An. gambiae. The relative expression of immune gene respect to control group (Sugar) was calculated using the Livak Method (Livak and Schmittgen, 2001).
Statistical analysis was performed using the Bio-Rad CFX Manager Software and the GraphPad software (http://www.graphpad.com). For each group, mean values from the biological replicates for each time-point were taken into account and the standard error (SEM) was calculated. One-way ANOVA test and the post-hoc test Dunn were used to assess the statistical differences between gene expressions in Asaia-challenged An. stephensi and An. gambiae mosquitoes and the presence of Plasmodium between treatments and controls. Differences in Asaia density among treatments over time and the gene expression in Asaia-challenged mosquitoes after uninfected or infected blood meal were calculated by two- way ANOVA test and the Bonferroni post-hoc test.
16S Miseq analysis was conducted on cDNA of An. stephensi mosquitoes fed on different diets by LGC Genomics (Berlin, Germany). The RNA came from the same mosquito described for the quantitative RT-PCR experiment. Briefly, the cDNA was amplified using the primers 341F and 785R targeting the region V3–V4 of 16S ribosomal RNA (Klindworth et al., 2013). Quality control of raw data was done using Mothur (Schloss et al., 2009) and then the sequences were searched for matching in the SILVA taxonomy database. OTUs diversity analysis was performed using QIIME software (Caporaso et al., 2010).
Asaia Colonization Activates the Basal Immune Levels in An. stephensi and An. gambiae
Despite the different concentrations of bacteria provided in the diet, Asaia quickly reached a similar homeostasis within 3 days in An. stephensi, where this bacterial species has been described as one of the main component of its natural microbiota (Figure 2). At the first time-point (1 day) sugar-fed and Asa4-fed mosquitoes showed similar Asaia density, compared to that detected in the cohort fed with Asa8 (p < 0.01): this early time-point is likely to reflect the quantity of Asaia administrated with the diets (Figure 2A). Between days 1 and 3, an increasing replication of Asaia in the control and Asa4-mosquitoes was observed, while Asa8-individuals showed constant bacterial density. At day 3, Asaia reached a similar homeostasis in all treatments, which was maintained during the following time-points, suggesting both adaptation of the bacterium and tolerance of the host (Figure 2A).
Figure 2 Gene expression and Asaia load in An. stephensi. Evaluation of Asaia load (A) at different time points and CEC1 (B), DEF1 (C), CTL4 (D), and TEP1 (E) genes expression. Asaia density (A) was normalized on RpS7 as a reference gene. The relative expression of CEC1, DEF1, CTL4, and TEP1 was normalized on RpS7 and compared to a calibrator (sugar group). Values represent the average ± SEM from two biological replicates. Differences between Asaia load in the groups were calculated by two-way ANOVA test and the Bonferroni post-hoc test. One-way ANOVA test and Dunn post-hoc test were used to calculate statistics between genes expression.*p < 0.05, **p < 0.01, ***p < 0.001.
For each time-point, the expression of CEC1, DEF1, CTL4, and TEP1 genes was assessed (Figures 2 B–E). After 24 h from Asaia administration, the expression of CTL4 resulted significantly up-regulated in Asa4 (p < 0.05) and Asa8 mosquitoes (p < 0.001) with respect to the control, and between the two concentrations of administrated Asaia (p < 0.01) (Figure 2D). Expression of the two analyzed AMPs appears to be differentially regulated. DEF1 expression is elicited by the lower concentration of Asaia reaching its maximal up-regulation at day 7, which coincides with the initial exponential phase of bacterial replication (Figure 2C). On the contrary, supplementation of higher concentrations of bacteria down-regulates DEF1 expression during the initial time points (Figure 2C).
CEC1 showed a delayed activation at day 10 after an initial down-regulation in Asa4-challenged samples. In contrast, higher doses of Asaia appeared to induce an earlier up-regulation of CEC1 between days 7 and 8, followed by its down-regulation from day 10 (Figure 2B). The TEP1 seemed to be marginally involved in the immune response against supplemented Asaia during the time window analyzed, except for being up-regulated in the Asa4 group after 12 days (Figure 2E).
Similarly to An. stephensi, females of An. gambiae were orally fed with the same concentrations of Asaia cells. Consistently with its role as a secondary component of the natural An. gambiae microbiota, Asaia doses are differently tolerated and regulated within the African malaria vector. A comparable homeostasis between doses is reached only after 7 days. Between 3 and 7 days, differences between bacteria-challenged mosquitoes appeared to be controlled and similarly stabilized: the persistence of Asaia in challenged individuals at the higher concentrations, compared to sugar-fed mosquitoes is maintained until the last time point where Asa4-fed mosquitoes mirrored the natural trend of sugar-fed individuals, whilst Asa8-colonized individuals experienced a significant drop in Asaia density (Figure 3A).
Figure 3 Gene expression and Asaia load in An. gambiae. Evaluation of Asaia load (A) at different time points and CEC1 (B), DEF1 (C), CTL4 (D), and TEP1 (E) genes expression. Asaia density (A) was normalized on RpS7 as a reference gene. The relative expression of CEC1, DEF1, CTL4, and TEP1 was normalized on RpS7 and compared to a calibrator (sugar group). Values represent the average ± SEM from two biological replicates. Differences between Asaia load in the groups were calculated by two-way ANOVA test and the Bonferroni post-hoc test. One-way ANOVA test and Dunn post-hoc test were used to calculate statistics between genes expression.*p < 0.05, **p < 0.01, ***p < 0.001.
Interestingly, in individuals of the group Asa8, the synergistic up-regulation of CEC1, DEF1, and CTL4 genes was observed during the initial time-points, probably elicited by the substantial colonization of the introduced bacteria (Figures 3B–D). In particular, CEC1 resulted to be initially up-regulated with respect to both groups (Figure 3B). DEF1 gene expression is characterized by a significant initial up-regulation during the early infection phase compared to the other groups (Figure 3C). Similarly, an up-regulation was detected in CTL4 expression level at the 1 day and 3, which, unlikely the AMPs expression pattern, resumed and persisted until day 10 (Figure 3D). The involvement of the effector of the complement system, TEP1, seemed to be limited to a minimal up-regulation on day 8 when compared to sugar-fed controls (p < 0.05) (Figure 3E).
In Asa4-challenged mosquitoes, the mounting of the immune response appeared delayed, starting after 3 days from Asaia administration, coinciding with the exponential bacterial replication at this time point (Figures 3B–E). The transcriptional activation of the two AMPs appeared to be similarly regulated during the initial infection phase, after which CEC1 up-regulation is observed (Figure 3B). Alike Asa8, CTL4 maintained its up-regulation from day 3 to day 8 compared to the sugar control (p < 0.05) in each time-point (Figure 3D). TEP1 resulted repetitively up-regulated compared to the control at day 3 (p < 0.01) and day 8 (p < 0.05), coinciding with the fluctuations in Asaia density.
Asaia-Induced Immune Response Reduces P. berghei in An. stephensi, but Not in An. gambiae
After 7 days of bacterial exposure, mosquitoes were blood fed with uninfected and P. berghei- infected blood, and the transcriptional activation of target immune genes was evaluated (Figures 4 and 5). In both mosquito species, the presence of Plasmodium in the blood meal of Asa4-challenged mosquitoes induced an increase in Asaia replication: in An. stephensi a peak in density was detected after 24 h (Figure 4A), while in An. gambiae is looks delayed (Figure 5A). When higher concentrations of Asaia are introduced (Asa8), a similar delay between mosquito species is observed (Figures 4B and 5B).
Figure 4 Effect of uninfected and P. berghei-infected blood meal on Asaia density and immune genes expression in An. stephensi. Evaluation of the fluctuations of Asaia density in mosquitoes challenged with the two doses of Asa4 (A) and Asa8 (B) and the related modulation of immune effectors after uninfected and infected blood meal (C, D, E, and F). Shown values represent the relative genes expression normalized on the reference gene RpS7 and against the calibrator represented by sugar-fed controls (relative expression of sugar-fed mosquitoes in Figure S1-A). The statistical differences of Asaia density and the expression level of the genes in the groups were calculated by two-way ANOVA test and the Bonferroni post-hoc test. *p < 0.05, **p < 0.01, ***p < 0.001.
Figure 5 Effect of uninfected and P. berghei-infected blood meal on Asaia density and immune genes expression in An. gambiae. Evaluation of the fluctuations of Asaia density in mosquitoes challenged with two doses of Asaia cells: Asa4 (A) and Asa8 (B), and the related modulation of immune effector genes after an uninfected and an infected blood meal (C, D, E, F). Shown values represent the relative genes expression normalized on the reference gene RpS7 and against the calibrator represented by sugar-fed controls (relative expression of sugar-fed mosquitoes in Figure S1-B). The statistical differences between Asaia density and the expression level of genes in the groups were calculated by two-way ANOVA test with Bonferroni post-hoc test. *p < 0.05, **p < 0.01, ***p < 0.001.
In An. stephensi, populations treated with Asaia-enriched diets do not show any particular activation of AMPs (Figures 4C, D) while the time window between days 10 and 12 coincides with the significant up-regulation of TEP1, often combined with CTL4, with both concentrations of Asaia, after an infected blood meal (Figures 4E, F).
The gene expression profiles for An. gambiae challenge with Asa4 revealed a very early activation at day 8, meaning 24 h after the blood meal, of CEC1 and DEF1, in Plasmodium-infected mosquitoes (Figures 5C, D). At the time point, in Plasmodium-infected Asa8-mosquitoes, do not show any particular activation of AMPs (Figures 5C, D). Interestingly, no up-regulation of TEP1 expression of infected-mosquitoes has been observed in both concentrations. Only CTL4 showed higher expression in infected mosquitoes challenged with Asa4 after 12 days (Figures 5E, F).
The hypothesis of a correlation between Plasmodium development and the colonization of Asaia at different concentrations was evaluated. Interestingly, in An. stephensi a significant reduction of Plasmodium ribosomal gene expression was detected in both treated groups (Asa4 and Asa8 groups) after 12 days (Figure 6A). The presence of the malaria parasite was also evaluated in An. gambiae: quantification of the parasite showed no significant reduction in Plasmodium replication, despite the activation of several immune genes (Figure 6B).
Figure 6 Plasmodium load in An. stephensi and An. gambiae mosquitoes challenged with Asaia. Evaluation of Plasmodium load has been performed at two time-points (three and five days after infected blood meal) in both An. stephensi (A) and An. gambiae (B). In the y axes the relative abundance of Plasmodium compared to the reference gene RpS7 is reported. Symbols in the plot represent individual mosquitoes (n = 9 per group of two experimental replicates, in total 18 mosquitoes) with horizontal lines indicating the medians (m). Statistical analysis was calculated with One-way ANOVA test and Dunn post-hoc test. **p < 0.01; ***p < 0.001.
An. stephensi Microbiota Abundance
The microbiota composition of An. stephensi fed on different diets was analyzed in order to directly correlate the immune response to a massive Asaia presence, especially in P. berghei infected mosquitoes where a high reduction of oocyst development was observed in mosquitoes infected with Asaia. At phylum level, Proteobacteria was the main predominant phylum present in all samples. Actinobacteria and Firmicutes were abundant in Sugar and Asa4 groups at 1 day and in 3 day only (Figure S2). Asaia represented the dominant genus of Proteobacteria phylum (Figure S3), reaching early the highest percentage in abundance in the mosquito populations that have been administrated with Asaia-enriched diets. After infected or uninfected blood meal, Asaia was the dominant bacteria in the mosquito populations with an OTUs abundance range between 70–90%.
The mosquito gut microbiota plays a crucial role in the host physiology contributing to the maintenance of metabolism and immunity homeostasis, but it can also stimulate a basal immune activity impacting on mosquito’s vector capacity (Dong et al., 2009). In fact, the introduction of special bacterial isolates in mosquitoes are able to trigger their innate immune response, which correlates with a decrease in the transmission of the malaria parasite (Frolet et al., 2006).
Although Asaia has already been described as able to stimulate the expression of some AMPs in mosquito while not being affected by phagocytosis (Capone et al., 2013), our results detailed the interactions between this bacteria and the mosquito immune system. We focused on some genes involved in Plasmodium surveillance: i) CEC1 and DEF1, belonging to AMPs gene families, are involved in the elimination of viruses, bacteria and Plasmodium (Bartholomay et al., 2004; Xi et al., 2008); ii) CTL4, encodes for C-type lectins that control the microbiota homeostasis (Hillyer, 2010; Pang et al., 2016); iii) TEP1, mainly involved in Plasmodium killing (Blandin et al., 2004; Dong et al., 2006). In particular, CLT4 and TEP1 act against the malaria parasite as agonists and antagonists, respectively. TEP1 together LRIM1 mediate the killing of ookinetes in the midgut epithelium; in contrast, CTL4 and the C-type lectin CTLMA2, protect the parasite inhibiting its melanization (Osta et al., 2004).
The supplementation of different concentrations of Asaia cells on newly emerged females showed distinctive effects in An. stephensi and An. gambiae. In An. stephensi, where the bacterium is among the dominant symbionts, Asaia quickly reached a persistent and consistent homeostasis in every experimental group. In Asa4 and Asa8 groups, the fluctuations of the bacterial load at day 1, until reaching the homeostasis at day 3, could be correlated to the up-regulation of the CTL4 gene, confirming its role in the regulation of the natural microbiota, in particular in relation to Gram-negative bacteria (Osta et al., 2004; Pang et al., 2016). Asaia density reached a constant plateau phase, remaining constant in both Asaia-challenged and control groups during later time points, possibly associated with the transcriptional induction of CEC1 and DEF1 genes.
In An. gambiae, Asaia showed to be differently regulated: likely its role as a secondary component of the natural microbiota of the African malaria vector could explain the difference in tolerance (Mancini et al., 2018). In fact, natural Asaia (sugar-fed control group) showed a gradual constant growth over time, while the infection with higher doses of cells underwent rapid fluctuations. This trend could be explained by the synergic action of the genes CEC1, TEP1, DEF1 and CTL4 in maintaining the microbiota balance. Concerning to the possible effect of bacterial challenges on Plasmodium infection, we have shown the ability of Asaia to activate the mosquito basal level immunity interfering with Plasmodium development in vivo. In fact, a significant reduction of malaria parasite load occurs five days after the infected blood meal, which coincides with stage when the parasite is present in midgut epithelium as premature oocysts (Wang and Jacobs-Lorena, 2013). The ability of Asaia to interfere with insect pathogens is corroborated by evidence in leafhopper as recently demonstrated by Gonella et al. (2019). The significant up-regulation of TEP1 in Asaia-challenged An. stephensi, despite the bacterial concentrations, could be correlated to its decrease in vector competence and indicates an indirect and exploitable interplay between Asaia and the parasite. Indeed, the contribution of the microbiota of the different modulations of the mosquito immune response, seems to be correlated just to the strong presence of Asaia as demonstrated by the 16S Miseq analysis, showing it as the most abundant bacterium in mosquito administrated with Asaia enriched diets.
The reduction of the parasite load observed in An. stephensi was not conserved in An. gambiae where the lack of activation of TEP1 in Asaia-challenged samples could explain the lack of Plasmodium inhibition in An. gambiae.
However, An. gambiae is not the natural vector of P. berghei, for which it is significantly more permissive than P. falciparum (Sinden et al., 2004). Moreover, An. gambiae mosquitoes showed a different transcriptional response to infection with P. berghei and P. falciparum (Dong et al., 2006). At light of consideration, further investigations on a possible Asaia role in immune stimulation in the system An. gambiae–P. falciparum are needed.
Nevertheless, these findings, while providing evidences on the ability of Asaia to stimulate the basal level of mosquito immunity in two main malaria vectors, and to naturally reduce the development of malaria parasite oocysts in An. stephensi. These findings confirm and expand its potential in SC approaches, not only through paratransgenesis, but also as a promising effector for mosquito immune priming.
The raw data supporting the conclusions of this manuscript will be made available by the authors, without undue reservation, to any qualified researcher.
All animal experiments were carried out according to the Italian Directive 116 of 10/27/92 on the “use and protection of laboratory animals” and in adherence with the European regulation (86/609) of 11/24/86, licence no. 125/94A, issued by the Italian Ministry of Health. The experiments were approved by the Ethic Committee of the University of Camerino (Protocol number 7/2014).
GF, MM, CD, and AC conceived and designed the experiments. GF supervised the project and gave conceptual advice. MM, CD, AC, MV, PR, AS, IR, and GF participated in the sample collection. MM, CD and AC performed the molecular analysis. GF and MM drafted the manuscript. GF, MM, CD, and AC edited the manuscript. All authors read and approved the final manuscript.
This study was supported by Grant PRIN 2012 (2012T85B3R_001) and 2015 (2015JXC3JF_001) from Italian Ministry of Education, University and Research both to GF; Grant FAR, Fondo di Ateneo alla Ricerca 2014 from the University of Camerino to GF.
Conflict of Interest Statement
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fgene.2019.00836/full#supplementary-material
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Keywords: Asaia, Plasmodium, malaria, symbiotic control, immune system
Citation: Cappelli A, Damiani C, Mancini MV, Valzano M, Rossi P, Serrao A, Ricci I and Favia G (2019) Asaia Activates Immune Genes in Mosquito Eliciting an Anti-Plasmodium Response: Implications in Malaria Control. Front. Genet. 10:836. doi: 10.3389/fgene.2019.00836
Received: 15 May 2019; Accepted: 13 August 2019;
Published: 25 September 2019.
Edited by:Jayme A. Souza-Neto, São Paulo State University, Brazil
Reviewed by:Jose Luis Ramirez, United States Department of Agriculture (USDA), United States
Marcos Henrique Ferreira Sorgine, Federal University of Rio de Janeiro, Brazil
Copyright © 2019 Cappelli, Damiani, Mancini, Valzano, Rossi, Serrao, Ricci and Favia. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Guido Favia, firstname.lastname@example.org
†Present address: Maria Vittoria Mancini, MRC-University of Glasgow-Centre for Virus Research, Glasgow, United Kingdom
‡Members of Centro Interuniversitario di Ricerca sulla Malaria