Expression of Human Mutant Huntingtin Protein in Drosophila Hemocytes Impairs Immune Responses

The pathogenic effect of mutant HTT (mHTT) which causes Huntington disease (HD) are not restricted to nervous system. Such phenotypes include aberrant immune responses observed in the HD models. However, it is still unclear how this immune dysregulation influences the innate immune response against pathogenic infection. In the present study, we used transgenic Drosophila melanogaster expressing mutant HTT protein (mHTT) with hemocyte-specific drivers and examined the immune responses and hemocyte function. We found that mHTT expression in the hemocytes did not affect fly viability, but the numbers of circulating hemocytes were significantly decreased. Consequently, we observed that the expression of mHTT in the hemocytes compromised the immune responses including clot formation and encapsulation which lead to the increased susceptibility to entomopathogenic nematode and parasitoid wasp infections. In addition, mHTT expression in Drosophila macrophage-like S2 cells in vitro reduced ATP levels, phagocytic activity and the induction of antimicrobial peptides. Further effects observed in mHTT-expressing cells included the altered production of cytokines and activation of JAK/STAT signaling. The present study shows that the expression of mHTT in Drosophila hemocytes causes deficient cellular and humoral immune responses against invading pathogens. Our findings provide the insight into the pathogenic effects of mHTT in the immune cells.

Introduction

Huntington's disease (HD) is an inherited neurodegenerative disorder caused by an abnormal expansion of CAG trinucleotide in the Huntingtin (htt) gene. Mutant HTT protein (mHTT) contains an extended polyglutamine tract encoded by 40 to over 150 CAG repeats, which causes cytotoxicity and leads to neurodegeneration; this results in involuntary movement, cognitive impairment, and psychiatric abnormalities (1). Although many clinical symptoms of HD are related to neuronal dysfunction, emerging evidence indicates that the expression of mHTT in non-neuronal cells of the brain or in the peripheral tissues also contributes to the pathogenesis of HD (2). Abnormal phenotypic effects caused by the dysfunction of non-neuronal cells have been described in cardiac cells, muscles, the endocrine system, adipose tissue, testes and immune cells of HD patients, and also in mouse HD models (2, 3).

Abnormalities related to the immune system were observed in a number of studies of HD patients (4). The expression of mHTT in both brain and peripheral immune cells (microglial and myeloid cells) induces the NF-κB signaling pathway which elevates levels of pro-inflammatory cytokines and chemokines, leading to systemic inflammation (5). In addition, macrophages isolated from HD model mice exhibited migration deficits, and microglia showed a delayed response to laser-induced injury in the brain (6). Although several studies proposed that the immune cell response is impaired in HD, this phenomenon is still poorly characterized in relation to host responses to pathogens. One recent study reported increased proliferation of a parasite, Toxoplasma gondii, in HD model mice, causing premature mortality and thus suggesting that expression of mHTT in immune cells may suppress immune responses (7).

Drosophila melanogaster has been long-term established as a HD model. In vivo experiments have revealed that the ectopic overexpression of mutant human htt (exon 1 with expanded CAG repeats) in the neural tissue of transgenic flies causes neurodegeneration (8, 9). The mechanisms of cellular pathology observed in the HD flies seem similar to those in human patients, including the suppression of mitochondrial function, transcriptional dysregulation, and neuronal apoptosis (10, 11). Genetic screening for disease modifiers in HD model flies led to the identification of the effects of sumoylation and HSP70 chaperone machinery on neurodegeneration. The subsequent confirmation that these pathways are involved in the pathology of human patients validates the Drosophila model for investigating HD (12, 13). Furthermore, since the tissue-specific expression of transgenes in Drosophila can be easily controlled using the UAS-Gal4 system, Drosophila have also been used to study the effects of HD on non-neuronal cells, including glial cells, photoreceptors, cardiac cells, and salivary glands (14–18).

The present study aimed to survey the physiological impact of mHTT expression in Drosophila hemocytes. We used the Drosophila UAS-Gal4 system to express mHTT with hemocyte-specific drivers and investigated the effect of mHTT on survival, hemocyte development, and susceptibility to pathogens. We also expressed mHTT in a Drosophila macrophage-like cell line, S2 cells, and assessed the effect of mHTT on phagocytic activity, ATP levels, antimicrobial peptides, and production of cytokines. Our results suggest that the expression of mHTT in hemocytes does not directly affect survival but causes immune dysregulation, which leads to an impaired immune response against pathogenic invasion.

Results

Expression of mHTT in Hemocytes Did Not Affect Larval Viability but Decreased the Number of Circulating Hemocytes

In order to characterize the effects of mHTT in Drosophila hemocytes, we used a tissue-specific UAS-Gal4 system by expressing wild-type human HTT (Q20) or mutant HTT (Q93) under the control of a pan-neuronal driver, elav-gal4, or hemocyte drivers, hml-gal4, and he-gal4. The flies devoid of plasmatocytes (phago^less) generated by expressing pro-apoptosis genes, rpr and hid with hml-gal4 were used as negative control (19, 20). The results showed that the ectopic expression of Q93 with the pan-neuronal driver (elav-gal4) decreased both the eclosion rate and the longevity of the adult flies, but not the rate of pupariation (Figure 1). The expression of Q20 and Q93 with both hemocyte drivers (hml-gal4 and he-gal4) had no effect on pupariation and eclosion rates. Furthermore, the differences in longevity between Q20 and Q93 flies were not significant, and their survival rate was higher than phago^less flies (Figure 1C). These results indicated that the hemocyte-specific expression of mHTT did not influence fly viability, unlike its expression in the brain.

FIGURE 1

Figure 1. The viability assays of mHTT-expressing flies under the control of the pan-neuronal driver (elav-gal4) and hemocyte drivers (hml-gal4 and he-gal4). (A) The effect of mHTT expression on pupariation (survival to pupal stage). (B) Eclosion (survival to adulthood) and (C) adult longevities were measured in control Q20 and mHTT Q93. All the experiments performed in at least six independent replicates. Data are presented as averages ± SEM. P-values for pupariation and eclosion rate using Student's t-test, ***P < 0.001, N.S., not significant. Significance analysis for longevity curve using weighted log-rank test.

Although the expression of mHTT did not affect fly survival, we observed a significant decrease in the number of circulating hemocytes. In first-instar larvae, the number of hemocytes differed significantly only in the phago^less flies (Figure 2A). However, a reduced amount of circulating and sessile hemocytes was apparent in the Q93 mutants from second-instar larvae. As shown in Figure 2B, the circular hemocyte numbers in Q93 larvae were still higher than in phago^less flies, showing about 50% of the numbers observed in the Q20 control (Figure 2B). These results showed that the expression of mHTT with two different hemocyte-specific drivers reduced the number of hemocytes.

FIGURE 2

Figure 2. Ectopic expression of mHTT decreased hemocyte numbers. (A) Microscope images indicated the decreased number of circulating and sessile hemocytes in mHTT-expressing second-instar larvae. Quantification of hemocytes by ectopic co-expression of HTT with GFP using hml-gal4 (B) or he-gal4 (C). Phago^less flies with hemocyte ablation (hml > UAS-rpr, hid) were used as a negative control. The number of the circular hemocyte corresponded to the total number of GFP positive cells in 25 μL of collected sample. At least five independent replicates were analyzed. Data are presented as averages ± SEM. Significances were analyzed by ANOVA with Fisher LSD post-hoc test (B), and the significant differences among treatment groups are marked with different letters (P < 0.05). Student's t-test was used for (C), ***P < 0.001.

Expression of mHTT in Hemocytes Impaired the Immune Response to Parasites

To examine whether mHTT expression in Drosophila hemocytes affects the innate immune response and whether such larvae are still able to restrain parasite development, we tested the sensitivity of such flies to entomopathogenic nematode and parasitoid wasp infections, which are two Drosophila pathogenic models for examining the cellular immune response (21, 22). Early third-instar larvae expressing mHTT (Q93), wild-type HTT (Q20) or phago^less were infected with nematode species, Heterorhabditis bacteriophora or Steinernema carpocapsae, which contain the bacterial symbionts Photorhabdus luminescens and Xenorhabdus nematophila, respectively. Mortality was calculated at 24 and 48 h post-infection. As shown in Figure 3, both phago^less and Q93 larvae displayed significantly higher mortality than Q20 controls. Previous studies revealed that the formation of hemolymph clot is an important innate immune response against entomopathogenic nematode infection in Drosophila (23, 24). To determine whether the expression of mHTT in the hemocytes caused clotting defects, we used an established bead aggregation assay (24, 25). Compared to the larvae expressing normal HTT (Q20), the hemolymph collected from mHTT (Q93)-expressing larvae displayed poor bead aggregation similar to phago^less larvae (Figure 3E). This results indicated that the expression of mHTT suppresses the clotting activity and thus increases the susceptibility to nematode infection.

FIGURE 3

Figure 3. Immune challenge with entomopathogenic nematode infection and clotting assay. Larvae expressing mHTT Q93 or HTT Q20 with hml-gal4 or he-gal4 hemocyte drivers were infected with H. bacteriophora (A,B), or S. carpocapsae (C,D). Mortality was calculated 24 and 48 h after infection. Phago^less flies with hemocyte ablation (hml > UAS-rpr, hid) were used as negative control. Bead aggregation assay was used for assessing the clotting activity (E). Hemolymph was collected from Q93, Q20, and Phago^less (hml-gal4) larvae, mixed with a bead suspension, and the aggregates were quantified by ImageJ software. All the experiments were performed in five to six independent replicates. Data are presented as averages ± SEM. Significances were analyzed by ANOVA with Fisher LSD post-hoc test; significant differences among treatment groups are marked with different letters (P < 0.05).

Similarly, we infected Drosophila larvae with a parasitoid wasp, Leptopilina boulardi and calculated the number of emerged fly and wasp adults. The number of eclosed Drosophila adults was not significantly different between Q20 and Q93 driven by hml-gal4 and he-gal4, while phago^less showed lower eclosion rates than both Q20 and Q93 (Figures 4A,B). However, the number of emerged wasps were significantly higher in both Q93 and phago^less flies, thus indicating that a greater number of wasps overwhelmed the immune reaction of Q93 hosts and successfully developed to adult stage. In addition, the higher number of wasp eggs successfully hatched in both Q93 and phagoless larvae (Figure 4C); these results indicated that Q93 and phago^less larvae have less efficient immune reaction against wasp infection. Since the encapsulation and melanization are major defense mechanisms against parasitoid wasp infection, we quantified the number of the melanized capsules to assess the immune activity after 72 h post-infection. We found that there were more intact melanized capsules in Q20 larvae (79%) than in those expressing Q93 (51.6%) or in phago^less (17.7%) (Figures 4D,G left). We also observed a higher amount of melanization pieces in Q93 or phago^less individuals than in Q20 larvae (Figures 4E,G middle). The formation of such defective capsules was described previously in immune-deficient mutant flies (26). Moreover, 37% of the infected phago^less larvae formed no melanization capsules compared to Q20 (0%) or Q93 (4.8%) infected larvae (Figures 4F,G right). These results could explain a lower proportion of phago^less adults successfully eclosed after wasp infection (Figures 4A,B). Taken together, our results suggest, that mHTT expression impairs the innate immune reactions to nematode and parasitoid wasp infections due to the deficient cellular immune responses such as clot formation and encapsulation.

FIGURE 4

Figure 4. Immune challenge with parasitoid wasp infection and encapsulation activity assay. Larvae expressing mHTT Q93 and HTT Q20 with hml-gal4 (A) or he-gal4 (B) hemocyte driver were infected with parasitoid wasp, L. boulardi. Phago^less flies (which underwent hemocyte ablation) were used as negative control. Thirty infected larvae were collected and the numbers of eclosed flies and wasps were calculated, indicating the number of flies overcoming the wasp infection and the number of wasps successfully escaping the fly's immune reaction, respectively. Data are presented as average ± SEM with more than 10 biological replicates. The significances of results for (A) were analyzed by ANOVA with a Fisher LSD post-hoc test; different letters on the treatment group indicate significant differences at P < 0.05. The significances of results for (B) were examined using Student's t-test, ***P < 0.001, N.S., not significant. For assessing the encapsulation activity, the numbers of fly larvae containing larvae of parasitic wasps (C), intact melanized capsules (D), melanized pieces (E) as well the numbers of the infected larvae without melanization (F) were recorded. The significances of the results were analyzed by Mann-Whitney U-test (paired); significant differences among treatment groups are marked with different letters (P < 0.05). The photos show examples of intact melanized capsule in Q20 larvae, melanized pieces in Q20 and Q93 larvae and infected phago^less without melanization reaction (G).

Reduced Phagocytic Activity and ATP Levels in mHTT Cells

To find out whether mHTT expression could cause a detrimental effect on hemocyte functions, we expressed mHTT or wild-type HTT in Drosophila S2 cells. The S2 cell line consists of macrophage-like cells with phagocytic activity and the ability to produce antimicrobial peptides (AMPs) (27). We transfected the cells with four different recombinant constructs encoding green fluorescent protein (GFP) fused to HTT repeats under an inducible metallothionein promoter. We created stable cell lineages and confirmed that the S2 cells expressed HTT-fusion proteins by observing the GFP. As shown in Supplemental Figure 1, most of the cells in all cell lineages were positive for the fluorophore. Furthermore, the cells containing the mHTT Q46, Q72, and Q97 constructs (all except wild-type Q25) showed formation of mHTT aggregates.

We further treated the HTT-expressing cells with E. coli particles conjugated by pH-sensitive dye (pHrodo) to examine their phagocytic activity. This causes bright fluorescence to be visible after particle engulfment in the acidic environment of phagolysosome. The results showed that after inducing mHTT expression, the fluorescence signals were significantly lower in Q46, Q72, and Q97 mHTT-expressing cells but not in cells expressing wild-type Q25 HTT (Figure 5A). Quantification of the cells containing fluorescent signals showed a significant reduction (20–30%) of fluorescent-positive cells in mHTT-expressing cells compared to the control cells (Q25) (Figure 5B), thus supporting the hypothesis that expression of mHTT in immune cells impairs phagocytic activity.

FIGURE 5

Figure 5. Impairment of phagocytic activities in mHTT-expressing S2 cells. S2 cell lineages expressing wild-type HTT (Q25) and mHTT (Q46, Q72, and Q97) were treated with pHrodo Red E. coli for 8 h. (A) Fluorescence microscope images show the decreased intensity of red fluorescence signals in mHTT-expressing cells. (B) The phagocytic rate was calculated as the percentage of cells showing a red fluorescence signal to the total number of cells in each image. Each treatment was performed in three independent replicates with (+copper) or without (–copper) CuSO₄ induction. Data are presented as average ± SEM. Significances were analyzed by ANOVA with Tukey HSD post-hoc test; different letters on the treatment group indicate significant differences at P < 0.05.

The phagocytic capacity of immune cells has been associated with mitochondrial activity (28–30); mHTT has been shown to cause impairment of energy metabolism and mitochondrial dysfunction in human peripheral blood cells (31). To test whether mHTT can also impair the energy metabolism of Drosophila immune cells, we measured the ATP levels in S2 lineages after mHTT induction. The results showed that ATP levels significantly decreased in cells expressing Q72 and Q97 mHTT after 72 h of induction (Figure 6A). The ATP levels in cells expressing Q46, Q72, and Q97 mHTT were further reduced after 120 h of induction (Figure 6B). This indicated that the expression of mHTT reduces ATP levels, which may further limit the cellular immune responses against pathogenic infection.

FIGURE 6

Figure 6. Decrease of ATP level and alternation of Bcl-2 protein expression in mHTT-expressing S2 cells. ATP levels of HTT- and mHTT-expressing S2 cells (5 × 10⁴ cells) were measured after 72 (A) and 120 h (B) of copper induction. Each treatment was performed in five independent replicates with (+copper) or without (–copper) copper induction. Data are presented as average ± SEM. Significances were analyzed by ANOVA with Tukey HSD post-hoc test; different letters on the treatment group indicate significant differences at P < 0.05. The mRNA levels of Drosophila Bcl-2 proteins, buffy and debcl were measured in Q25 HTT and Q97 mHTT-expressing S2 cells after 120 h of induction (C). All the expressions were normalized to rp49 transcript and Q25 control (ΔΔCT). Data are presented as average ± SEM from three independent replicates. P-values were determined using Student's t-test, ***P < 0.001.

The studies in human and mouse have demonstrated that the expression of Bcl-2 family proteins associated with mitochondrial dysfunction is activated by mHTT expression (32). To assess whether the level of Drosophila Bcl-2 proteins is also altered by mHTT expression, we compared the transcription levels of two of Bcl-2 genes, buffy and debcl, in Q25- and Q97- expressing S2 cells (Figure 6C). We found that buffy expression is five times higher in Q97- than in Q25- expressing cells, but we did not detect any significant difference in debcl mRNA level. Different from pro-apoptotic function of debcl, buffy was suggested to play an anti-apoptotic role under stress conditions which is similar to mammalian Bcl-2 proteins (33, 34). We conclude that the alternation of ATP synthesis and buffy expression indicate the abnormality of mitochondrial function in mHTT expressing cells, and the induction of buffy might be a protective mechanism for preventing the cell death caused by mitochondrial dysfunction.

Upregulation of Cytokines Expression and Downstream JAK/STAT Signaling in mHTT Expression Cells

It has been reported that the level of cytokines and chemokines are abnormally increased in the plasma of HD patients (35). Consistently, the production of cytokines from monocytes and macrophages of HD patients have shown hyper-activation after lipopolysaccharide stimulation (36). To test whether mHTT has a similar effect in Drosophila, we used Schneider 2 (S2) cells and measured the effect of mHTT expression on three Drosophila cytokines, upd1, upd2, and upd3, as well as dome, jak (hop) and downstream targets of JAK-STAT signaling (Figure 7A). The results showed that the expression of cytokine upd3 is significantly increased in Q97 mHTT-expressing cells compared to Q25 controls (Figure 7B). In addition, the expression of dome receptor and four downstream targets, tep1, totA, totB, and totC were also significantly increased in Q97-expressing cells. These results indicated that the expression of mHTT induced the production of cytokines and activates JAK/STAT signaling.

FIGURE 7

Figure 7. Activation of cytokine expression and JAK/STAT signaling in the mHTT-expressing S2 cells. (A) Schematic representation of the interaction between Upds and JAK/STAT pathway. (B) The gene expression of cytokines (udp1-3), dome, jak(hop), and JAK/STAT downstream target genes (teps and tots) were measured in Q25 HTT and Q97 mHTT-expressing S2 cells after 120 h of copper induction. All the expressions were normalized to rp49 expression and Q25 control (ΔΔCT). Data are presented as average ± SEM from three independent replicates. P-values using Student's t-test, *P < 0.05, ***P < 0.001.

Decreased Antimicrobial Peptide (AMP) Production in Response to Bacteria

Drosophila Toll and Imd pathways control the humoral immune response against invasive microorganisms by regulating the induction of downstream AMP genes in both hemocytes and the fat body (37). To examine whether AMP induction was affected by mHTT expression in Drosophila S2 cells, we treated mHTT-expressing cells with a mixture of heat-inactivated Gram-negative bacteria, Escherichia coli, and Gram-positive bacteria, Micrococcus luteus. The induction of AMPs was assessed using qPCR. As shown in Figure 8, there was no difference in the expression of AMPs between Q25 and Q97 in the absence of bacterial treatment. In contrast, all AMP genes were significantly induced in both Q25- and Q97-expressing cells at 8 h after bacterial treatment. However, AMP induction levels were significantly lower in cells expressing Q97 (Figure 8A). We further assessed the AMP expression levels under in vivo condition after infecting larvae with phytopathogenic bacteria, Erwinia carotovora carotovora 15 (Ecc15). We examined the expression levels of dpt, dptB, attA, and cecA which were known as being highly induced after Ecc15 infection (38). Our results of larval infections showed that except for attA, the induction levels of dpt, dptB, and cecA in Q93 or phago^less larvae were significantly lower than in Q20 controls (Figure 8B). These results confirm that the induction of AMPs in response to bacteria was significantly suppressed in mHTT-expressing cells or larvae.

FIGURE 8

Figure 8. Suppression of antimicrobial peptides (AMPs) induction after bacterial treatment in the mHTT-expressing S2 cells and larvae. (A) Q25 and Q97-expressing S2 cells were incubated with E. coli and M. luteus (Q25_B and Q97_B) or without bacteria (Q25_C and Q97_C) for 8 h, and the expression levels of AMPs was measured. The AMPs expressions were normalized to rp49 expression and Q25 control. (B) Larvae expressing mHTT Q93 or HTT Q20 under hml-gal4 hemocyte drivers as well as Phago^less mutants were infected with ECC15-GFP and their expression of AMPs was determined after 8 h. The expressions were normalized to rp49 transcripts and non-infected controls. The AMPs expression levels of non-infected controls for each genotype were set to one. All the data are presented as average ± SEM from three independent replicates. The significances were analyzed by ANOVA with Fisher LSD post-hoc test; different letters on the treatment group indicate significant differences at P < 0.05.

Discussion

Peripheral immune dysregulation is considered as one of the clinical features of HD pathogenesis (39). Previous studies in mice and HD patients have suggested that mHTT expression in immune cells accelerates the neurodegenerative process. The activation of pro-inflammatory products in mHTT-expressing microglial cells elevate the reactive oxygen species (ROS) and cause neuroinflammation, which contributes to neurodegeneration (5, 40). Genetic ablation or pharmacologically-blocked cannabinoid receptor 2 (interleukin-6 regulator), as well as drug suppression of the cytokine-responsive kynurenine pathway, can both slow neurodegeneration and improve the phenotype of R6/2 HD mice (41, 42). Since the expression of mHTT in HD mice and human patients is ubiquitous, it is still unclear whether mHTT expression in blood cells directly contributes to the lethal effect of HD. The present study examined mHTT expressed specifically in Drosophila blood cells and assessed its impacts on development and longevity (Figure 1). We found that the expression of mHTT in hemocytes did not cause mortality or a shortening in life span, which is in contrast to expression in the brain. Our results, therefore, suggest that expression of mHTT in immune cells does not directly contribute to mortality.

A reduced proliferation of immune cells has been observed in T. gondii-infected HD mice, in which the expansion of CD8⁺ T-cells in the spleen and brain was significantly suppressed during infection (7). Our results showed that the expression of mHTT in flies with hemocyte-specific drivers causes a significant reduction in the number of circulating hemocytes (Figure 2), and this decrease might be caused by dysfunction of mitochondria (Figure 7). The mitochondrial abnormalities resulting in metabolic dysregulation in peripheral blood cells of HD patients increase oxidative damage and suppress their anti-oxidant capacity (40). The activation of caspase-3 and caspase-9 in lymphoblasts of HD patients increases apoptosis under stress conditions (43).

The mHTT-expressing larvae revealed a higher susceptibility to wasp and nematode infections and this phenotype was caused by defects of clot formation and encapsulation (Figures 3, 4). It has been shown that wasp egg recognition by circulating plasmatocytes and their differentiation to lamellocytes for further encapsulation are important processes of the immune response against wasp invasion in Drosophila (44). The production of clotting components from hemocytes also contributes to wound healing and melanization, which are important against nematode or wasp infections (24, 45). mHTT-expressing macrophages and monocytes from HD mice and patients also showed migration defects toward an inflammatory stimulus (6). Hemocyte migration and adhesion are important factors for the development of embryonic macrophages, as well as successful wound healing and encapsulation during wasp infection (46). Furthermore, decreased phagocytic activity toward bacterial particles (Figure 5) and a suppressed induction of antimicrobial peptides (Figure 8) can also contribute to immune deficiency against the bacterial symbionts of nematodes (23, 47).

A previous study showed that macrophages isolated from HD patients and R6/2 mice displayed increased phagocytosis when incubated with fluorescent polystyrene beads (48). Our results seemingly differ because we observed reduced phagocytic activity of the Drosophila macrophage-like cells expressing different mHTT fragments (Figure 5). Unlike their approach, we tested phagocytic activity using E. coli particles with a pH-sensitive fluorescent dye that can accurately confirm phagosome formation and initiation of the phagolysosome acidification. However, similar to their results, we found that S2 cells expressing mHTT were able to initiate phagocytosis. We tested this by treating the S2 cells with heat-inactivated E. coli labeled with DNA-specific fluorescent dye (without pH-sensor); the results showed that mHTT-expressing cells were indeed able to engulf E. coli (Supplemental Figure 2). Thus, our results suggest that mHTT-expressing cells were unable to complete the process of phagocytosis to final phagolysosome acidification. In addition, a defective actin function has been reported in HD mouse immune cells leading to failure of membrane ruffling (6), which supports our results since actin assembly is required to trigger engulfment and phagolysosome maturation for successful phagocytosis (49).

Consistent with previous observations in HD mice and patients, we also found that Drosophila hemocyte cytokine udp3 was upregulated in mHTT-expressing cells (Figure 8). Udp3 binds to the JAK/STAT signaling receptor, Dome, and initiates phosphorylation cascades which translocate the transcription factor, Stat92E, into the nucleus and activates downstream target genes (Figure 7A) (50). Two selected downstream target genes, tep1 and totA, were highly expressed in mHTT-expressing cells (Figure 7B). Notably, we found that the induction of antimicrobial peptides was significantly suppressed in mHTT-expressing cells after bacterial treatments, which has not yet been observed in other HD models. It is known that several human antimicrobial peptides are expressed in blood cells including neutrophils and macrophages (51). Since the transcriptomic analysis in HD blood cells has shown dysregulation of transcription in large genomic regions (52), further studies will be needed to understand whether the production of antimicrobial peptides is impaired in the blood cells of patients or HD mice during infection.

In summary, the present study demonstrates immune dysregulation in flies expressing mHTT in hemocytes (Figure 9). This expression does not directly cause a lethal effect, although it does reduce the number of circulating hemocytes and decrease ATP levels. Cytokine expression and downstream JAK/STAT signaling are activated upon mHTT expression, which has also been observed in HD patients and mice. In addition, the induction of antimicrobial peptides as well as the immune response against different pathogenic infections are impaired in mHTT-expressing Drosophila cells. The present study introduces a system for studying the tissue-specific effects of mHTT in Drosophila immune cells. Further studies can be applied to clarify the molecular interaction between mHTT and antimicrobial peptide pathways (Toll and IMD signaling) as well as the mechanisms of phagocytosis suppression.

FIGURE 9

Figure 9. Model of mHTT effects on Drosophila and mammalian immune cells. The expression of mHTT in hemocytes of Drosophila displays similar effects on the immune cells of HD patients and mice.

Materials and Methods

Fly Stocks

Flies were reared at 25°C on standard cornmeal medium. The fly strains used were UAS-Q20Httexon1^111F1L and UAS-Q93Httexon1^4F132 obtained from Prof. Lawrence Marsh (UC Irvine, USA) (8), which contain 20 (wild-type) and 93 (mutant HTT) polyglutamine repeats, respectively. The pan-neuronal driver, elav-gal4[C155], and hemocyte drivers, he-gal4 and hml-gal4, were obtained from Bloomington Drosophila Stock Center and Dr. Tomas Dolezal (University of South Bohemia), respectively (53–55). Hemocyte-ablated flies (phago^less) were used as negative controls and were generated by overexpressing pro-apoptotic proteins (UAS-rpr, -hid) with hml-gal4 (19, 20, 56).

Developmental and Longevity Assay

Thirty first-instar larvae collected from a juice plate were transferred into vials to measure the number of pupae and adults for each replicate. For the longevity assay, about 20–30 newly emerged male adults were collected for each replicate and maintained at 29°C. Q93 expression driven by pan-neuronal driver, elav-gal4 and phgo^less flies were used as positive controls for longevity assay. Since expression of Q93 driven by elav-gal4 (X chromosome insertion) results in high mortality of male progeny (dosage compensation) (57), female progeny were used for recording the longevity. The number of dead flies was counted every day. All the experiments were performed in at least six independent replicates.

Circulating Hemocyte Counting

Circulating hemocytes were obtained from larvae by cuticle tearing in Ringer's buffer with thiourea to prevent melanization (25 μl of buffer per 6 larvae). The number of hemocytes expressing GFP (hml-gal4 or he-gal4 > UAS-gfp) were counted using a hemocytometer. At least five independent replicates were analyzed for each genotype.

Parasitoid Wasp Infection, Eclosion, and Encapsulation Assay

Leptopilina boulardi parasitoid wasps were obtained from Dr. Jan Hrček (Biology Center CAS) and maintained by infecting wild-type Drosophila larvae. For the wasp infection assay, forty larvae (second instar) were transferred onto a dish containing cornmeal food, and three female wasps were then placed onto the dish and allowed to attack for 72 h. After infection, 30 infected larvae were collected from the dish and transferred into a vial containing cornmeal for each replicate. Each genotype was tested in at least 10 independent replicates. The total number of eclosed flies and wasps were calculated (26). For the encapsulation assay, the infected larvae were dissected 72 h post-infection and the number of larvae containing intact melanized capsules, broken melanized pieces as well as wasp larvae was recorded.

Nematode Infection

Two nematode species, Steinernema carpocapsae and Heterorhabditis bacteriophora, were used in this study, under previously described maintenance conditions (58). For the infection assay, nematodes were combined with autoclaved water to achieve a concentration of 25 infective juveniles per 10 μl. Then, 10 μl of nematode suspension was applied to paper and placed in each wells of a 96-well plate. Individual larvae were transferred to each well where they stayed in contact with the nematodes, and the plate was covered with Parafilm. The infection was conducted at 25°C in the dark. Each experimental replicate consisted of 32 early third-instar larvae (72 h after egg hatching), and all experiments were done at least in five replicates. The number of dead larvae were counted after 24 and 48 h of infection (23, 24).

Bead Aggregation Assay

The bead aggregation assay was described in our previous study (24). Briefly, 2.5 μl of hemolymph was collected from six late third-instar larvae, mixed with BSA-blocked bead suspension (tosylactivated Dynabeads M-280, Invitrogen), diluted in Drosophila Ringer (pH 6.0) in a well of cavity diagnostic slide (Thermo Scientific) and covered with round cover glass. Pictures were taken with a Nikon SMZ-745T stereomicroscope associated with a CANON EOS 550D. The images were analyzed and quantified with the ImageJ graphics software with the “Analyze Particles” module.

Cell Culture

Drosophila Schneider 2 (S2) cells were grown at 25°C in Shields and Sang medium (Sigma) with 0.1% yeast extract, 0.25% peptone, and 10% heat inactivated fetal bovine serum. To generate stable lines expressing polyglutamine repeats, the S2 cells were transfected with four different Httex1-eGFP pMK33 plasmids (Q25, Q46, Q72, and Q97) containing copper-inducible metallothionein promoter (obtained from Dr. Sheng Zhang) (59).

Phagocytosis Assay

After induction for 5 days (120 h) with 1 mM copper (CuSO₄; Sigma), 100 μl of cell suspension (1 × 10⁶ cells/ml) was transferred to each well of a 96-well plate. Then, 100 μl of pHrodo Red E. coli (1 mg/ml; Thermo Fisher Scientific) was applied to each well for phagocytosis testing. After 8 h of treatment, the supernatant was removed, the cells were washed two times with 1× PBS, and 100 μl of fresh medium was applied. Cells were observed and photographed with a confocal microscope. From the images, the total number of cells and the number of cells displaying red fluorescence were counted. Three experimental repeats for each treatment were done for statistical analysis.

ATP Measurement

Cells were treated with 1 mM copper for 3 days (72 h) and 5 days (120 h) to induce mHTT expression. Fifty microliter of a 1 × 10⁶ cells/ml solution (5 × 10⁴ cells) was transferred to each well of a 96-well plate. After removing the supernatant, 60 μl of CellTiter-Glo solution (Promega) was applied to each well for 10 min. Then, 50 μl of the mixture was transferred to each well of 96-well white plates and the intensity of luminescence was then measured. Five independent replicates for each treatment were performed for analysis.

Bacterial Infection in vitro and in vivo

Five milliliter of S2 cells (1 × 10⁶ cells/ml) carrying copper-inducible Q25 HTT or Q97 mHTT transgenes were incubated in media containing 1 mM CuSO₄ for 120 h in 60 mm tissue culture plates. After the induction, the cells were treated for 8 h with 1 ml of bacterial mixture containing Escherichia coli and Micrococcus luteus at an optical density (600 nm) of 1 (OD₆₀₀ = 1) (37). The cells were then harvested for RNA extraction.

For the in vivo infection, late third instar larvae (96 h after egg hatching) were collected and transferred into a vial with 0.5 g instant Drosophila medium (Formula 4–24, Carolina Biological Supply) supplemented with 200 μl of bacterial suspension (OD₆₀₀ = 50) Erwinia carotovora carotovora 15-GFP (ECC15-GFP) and 1,300 μl of distilled water. The larvae were collected for RNA extraction 8 h after the infection (19, 38).

RNA Extraction

For in vitro experiments, S2 cells were washed with 1× PBS three times and harvested with 800 μl of RiboZol (VWR). Samples were preserved at −80°C until RNA purification. For in vivo experiments, 10 larvae were washed by distilled water and homogenized by the pestle motor (Kimble) in 200 μl of RiboZol (VWR Life Science). The sample were then preserved at −80°C for further RNA purification. RNA was isolated using NucleoSpin RNA columns (Macherey-Nagel) following the manufacturer's instructions and cDNA was synthesized from 2 μg of total RNA using a RevertAid H Minus First Strand cDNA Synthesis Kit (Thermo Fisher Scientific).

qPCR and Primers

5× HOT FIREPol^® EvaGreen^® qPCR Mix Plus with ROX (Solis Biodyne) and an Eco Real-Time PCR System (Illumina^®) were used for qPCR. The cDNA was diluted 50 times before use. Each reaction contained 4 μl of EvaGreen qPCR mix, 0.5 μl of forward and reverse primer (10 μM), 5 μl of diluted cDNA and ddH2O to adjust the total volume to 20 μl. The list of primers is shown in Supplemental Table 1. The expression level was calculated by using the (2^−ΔΔCT) method. The CT value of target genes were normalized to reference gene, ribosomal protein 49 (rp49).

Statistical Analysis

Error bars show standard error of the mean throughout this paper. Significance was established using Student's t-test (N.S., not significant, *P < 0.05, **P < 0.01, ***P < 0.001) or one-way ANOVA analysis with Fisher LSD or Tukey HSD post-hoc test. The Mann–Whitney U-test was used for examing the significance of the data on wasp larval hatching and the host encapsulation activities (Figures 4C–F). For the statistical analysis of longevity curve, we used online tool OASIS 2 to perform the weighted log-rank test for determining significance (60).

Data Availability Statement

The raw data supporting the conclusions of this manuscript will be made available by the authors, without undue reservation, to any qualified researcher.

Author Contributions

Y-HL conceived the project, performed the experiments and prepared the manuscript. HM performed the hemocyte counting and imaging. EI performed the nematode infections. LK performed the clotting assay. MZ supervised the project and manuscript preparation.

Funding

This work was supported by the grant agency of the University of South Bohemia (065/2017/P to Y-HL), junior grant project GACR (19-13784Y to LK). MZ was a member of the COST action Maximizing impact of research in neurodevelopmental disorders (CA16210).

Conflict of Interest

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.

Acknowledgments

We thank Dr. Sheng Zhang (UThealth) for the Httex1-eGFP pMK33 plasmids, Prof. L. Marsh (UC Irvine, USA) for Q20 and Q93 flies, Dr. Tomas Dolezal (University of South Bohemia) for the hemocyte driver line, Dr. Pavel Hyrsl, Pavel Dobes (Masaryk University) for the nematodes, and Dr. Hrcek Jan, Dr. Chia-Hua Lue (Biology Centre CAS), and Dr. Adam Bajgar (University of South Bohemia) for the parasitoid wasps, Dr. Julien Royet (IBDM, France) for bacteria ECC-15.

Supplementary Material

The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fimmu.2019.02405/full#supplementary-material

Supplemental Figure 1. Expression of four different lengths of HTT-GFP fusion proteins under a fluorescence microscope. mHTT-expressing cells (Q46, Q72, and Q97) showed significant mHTT aggregates after copper induction, while there was no aggregate formation in normal HTT-expressing cells (Q25).

Supplemental Figure 2. Phagocytosis assay in Q25- and Q97-expressing S2 cells with E. coli labeled by DNA-specific dye (Hoechst 33342). Cells expressing mHTT were able to initiate phagocytosis.

Supplemental Table 1. List of qPCR primers used in this study.

References

1. Vonsattel JP, DiFiglia M. Huntington disease. J Neuropathol Exp Neurol. (1998) 57:369–84. doi: 10.1097/00005072-199805000-00001

PubMed Abstract | CrossRef Full Text | Google Scholar

2. Sassone J, Colciago C, Cislaghi G, Silani V, Ciammola A. Huntington's disease: the current state of research with peripheral tissues. Exp Neurol. (2009) 219:385–97. doi: 10.1016/j.expneurol.2009.05.012

PubMed Abstract | CrossRef Full Text | Google Scholar

3. Sathasivam K, Hobbs C, Turmaine M, Mangiarini L, Mahal A, Bertaux F, et al. Formation of polyglutamine inclusions in non-CNS tissue. Hum Mol Genet. (1999) 8:813–22. doi: 10.1093/hmg/8.5.813

PubMed Abstract | CrossRef Full Text | Google Scholar

4. Leblhuber F, Walli J, Jellinger K, Tilz GP, Widner B, Laccone F, et al. Activated immune system in patients with Huntington's disease. Clin Chem Lab Med. (1998) 36:747–50. doi: 10.1515/CCLM.1998.132

PubMed Abstract | CrossRef Full Text | Google Scholar

5. Andre R, Carty L, Tabrizi SJ. Disruption of immune cell function by mutant huntingtin in Huntington's disease pathogenesis. Curr Opin Pharmacol. (2016) 26:33–8. doi: 10.1016/j.coph.2015.09.008

PubMed Abstract | CrossRef Full Text | Google Scholar

6. Kwan W, Trager U, Davalos D, Chou A, Bouchard J, Andre R, et al. Mutant huntingtin impairs immune cell migration in Huntington disease. J Clin Invest. (2012) 122:4737–47. doi: 10.1172/JCI64484

PubMed Abstract | CrossRef Full Text | Google Scholar

7. Donley DW, Olson AR, Raisbeck MF, Fox JH, Gigley JP. Huntingtons disease mice infected with Toxoplasma gondii demonstrate early kynurenine pathway activation, altered CD8⁺ T-cell responses, and premature mortality. PLoS ONE. (2016) 11:e0162404. doi: 10.1371/journal.pone.0162404

PubMed Abstract | CrossRef Full Text | Google Scholar

8. Steffan JS, Bodai L, Pallos J, Poelman M, McCampbell A, Apostol BL, et al. Histone deacetylase inhibitors arrest polyglutamine-dependent neurodegeneration in Drosophila. Nature. (2001) 413:739–43. doi: 10.1038/35099568

PubMed Abstract | CrossRef Full Text | Google Scholar

9. Song W, Smith MR, Syed A, Lukacsovich T, Barbaro BA, Purcell J, et al. Morphometric analysis of Huntington's disease neurodegeneration in Drosophila. Methods Mol Biol. (2013) 1017:41–57. doi: 10.1007/978-1-62703-438-8_3

PubMed Abstract | CrossRef Full Text | Google Scholar

10. Taylor JP, Taye AA, Campbell C, Kazemi-Esfarjani P, Fischbeck KH, Min KT. Aberrant histone acetylation, altered transcription, and retinal degeneration in a Drosophila model of polyglutamine disease are rescued by CREB-binding protein. Genes Dev. (2003) 17:1463–8. doi: 10.1101/gad.1087503

PubMed Abstract | CrossRef Full Text | Google Scholar

11. Li XJ, Orr AL, Li S. Impaired mitochondrial trafficking in Huntington's disease. Biochim Biophys Acta. (2010) 1802:62–5. doi: 10.1016/j.bbadis.2009.06.008

PubMed Abstract | CrossRef Full Text | Google Scholar

12. Warrick JM, Chan HY, Gray-Board GL, Chai Y, Paulson HL, Bonini NM. Suppression of polyglutamine-mediated neurodegeneration in Drosophila by the molecular chaperone HSP70. Nat Genet. (1999) 23:425–8. doi: 10.1038/70532

PubMed Abstract | CrossRef Full Text | Google Scholar

13. Steffan JS, Agrawal N, Pallos J, Rockabrand E, Trotman LC, Slepko N, et al. SUMO modification of Huntingtin and Huntington's disease pathology. Science. (2004) 304:100–4. doi: 10.1126/science.1092194

PubMed Abstract | CrossRef Full Text | Google Scholar

14. Marsh JL, Walker H, Theisen H, Zhu YZ, Fielder T, Purcell J, et al. Expanded polyglutamine peptides alone are intrinsically cytotoxic and cause neurodegeneration in Drosophila. Hum Mol Genet. (2000) 9:13–25. doi: 10.1093/hmg/9.1.13

PubMed Abstract | CrossRef Full Text | Google Scholar

15. Tamura T, Sone M, Yamashita M, Wanker EE, Okazawa H. Glial cell lineage expression of mutant ataxin-1 and huntingtin induces developmental and late-onset neuronal pathologies in Drosophila models. PLoS ONE. (2009) 4:e4262. doi: 10.1371/journal.pone.0004262

PubMed Abstract | CrossRef Full Text | Google Scholar

16. Besson MT, Dupont P, Fridell YW, Lievens JC. Increased energy metabolism rescues glia-induced pathology in a Drosophila model of Huntington's disease. Hum Mol Genet. (2010) 19:3372–82. doi: 10.1093/hmg/ddq249

PubMed Abstract | CrossRef Full Text | Google Scholar

17. Weiss KR, Kimura Y, Lee WC, Littleton JT. Huntingtin aggregation kinetics and their pathological role in a Drosophila Huntington's disease model. Genetics. (2012) 190:581–600. doi: 10.1534/genetics.111.133710

PubMed Abstract | CrossRef Full Text | Google Scholar

18. Melkani GC, Trujillo AS, Ramos R, Bodmer R, Bernstein SI, Ocorr K. Huntington's disease induced cardiac amyloidosis is reversed by modulating protein folding and oxidative stress pathways in the Drosophila heart. PLoS Genet. (2013) 9:e1004024. doi: 10.1371/journal.pgen.1004024

PubMed Abstract | CrossRef Full Text | Google Scholar

19. Charroux B, Royet J. Elimination of plasmatocytes by targeted apoptosis reveals their role in multiple aspects of the Drosophila immune response. Proc Natl Acad Sci USA. (2009) 106:9797–802. doi: 10.1073/pnas.0903971106

PubMed Abstract | CrossRef Full Text | Google Scholar

20. Defaye A, Evans I, Crozatier M, Wood W, Lemaitre B, Leulier F. Genetic ablation of Drosophila phagocytes reveals their contribution to both development and resistance to bacterial infection. J Innate Immun. (2009) 1:322–34. doi: 10.1159/000210264

PubMed Abstract | CrossRef Full Text | Google Scholar

21. Dobes P, Wang Z, Markus R, Theopold U, Hyrsl P. An improved method for nematode infection assays in Drosophila larvae. Fly. (2012) 6:75–9. doi: 10.4161/fly.19553

PubMed Abstract | CrossRef Full Text | Google Scholar

22. Small C, Paddibhatla I, Rajwani R, Govind S. An introduction to parasitic wasps of Drosophila and the antiparasite immune response. J Vis Exp. (2012) 63:e3347. doi: 10.3791/3347

CrossRef Full Text | Google Scholar

23. Arefin B, Kucerova L, Dobes P, Markus R, Strnad H, Wang Z, et al. Genome-wide transcriptional analysis of Drosophila larvae infected by entomopathogenic nematodes shows involvement of complement, recognition and extracellular matrix proteins. J Innate Immun. (2014) 6:192–204. doi: 10.1159/000353734

PubMed Abstract | CrossRef Full Text | Google Scholar

24. Kucerova L, Broz V, Arefin B, Maaroufi HO, Hurychova J, Strnad H, et al. The Drosophila chitinase-like protein IDGF3 is involved in protection against nematodes and in wound healing. J Innate Immun. (2016) 8:199–210. doi: 10.1159/000442351

PubMed Abstract | CrossRef Full Text | Google Scholar

25. Lesch C, Goto A, Lindgren M, Bidla G, Dushay MS, Theopold U. A role for Hemolectin in coagulation and immunity in Drosophila melanogaster. Dev Comp Immunol. (2007) 31:1255–63. doi: 10.1016/j.dci.2007.03.012

PubMed Abstract | CrossRef Full Text | Google Scholar

26. Mortimer NT, Kacsoh BZ, Keebaugh ES, Schlenke TA. Mgat1-dependent N-glycosylation of membrane components primes Drosophila melanogaster blood cells for the cellular encapsulation response. PLoS Pathog. (2012) 8:e1002819. doi: 10.1371/journal.ppat.1002819

PubMed Abstract | CrossRef Full Text | Google Scholar

27. Ramet M, Manfruelli P, Pearson A, Mathey-Prevot B, Ezekowitz RA. Functional genomic analysis of phagocytosis and identification of a Drosophila receptor for E. coli Nature. (2002) 416:644–8. doi: 10.1038/nature735

CrossRef Full Text | Google Scholar

28. West AP, Brodsky IE, Rahner C, Woo DK, Erdjument-Bromage H, Tempst P, et al. TLR signalling augments macrophage bactericidal activity through mitochondrial ROS. Nature. (2011) 472:476–80. doi: 10.1038/nature09973

PubMed Abstract | CrossRef Full Text | Google Scholar

29. Chougnet CA, Thacker RI, Shehata HM, Hennies CM, Lehn MA, Lages CS, et al. Loss of phagocytic and antigen cross-presenting capacity in aging dendritic cells is associated with mitochondrial dysfunction. J Immunol. (2015) 195:2624–32. doi: 10.4049/jimmunol.1501006

PubMed Abstract | CrossRef Full Text | Google Scholar

30. Geng J, Sun X, Wang P, Zhang S, Wang X, Wu H, et al. Kinases Mst1 and Mst2 positively regulate phagocytic induction of reactive oxygen species and bactericidal activity. Nat Immunol. (2015) 16:1142–52. doi: 10.1038/ni.3268

PubMed Abstract | CrossRef Full Text | Google Scholar

31. Ehinger JK, Morota S, Hansson MJ, Paul G, Elmer E. Mitochondrial respiratory function in peripheral blood cells from Huntington's disease patients. Mov Disord Clin Pract. (2016) 3:472–82. doi: 10.1002/mdc3.12308

PubMed Abstract | CrossRef Full Text | Google Scholar

32. Sassone J, Maraschi A, Sassone F, Silani V, Ciammola A. Defining the role of the Bcl-2 family proteins in Huntington's disease. Cell Death Dis. (2013) 4:e772. doi: 10.1038/cddis.2013.300

PubMed Abstract | CrossRef Full Text | Google Scholar

33. Quinn L, Coombe M, Mills K, Daish T, Colussi P, Kumar S, et al. Buffy, a Drosophila Bcl-2 protein, has anti-apoptotic and cell cycle inhibitory functions. EMBO J. (2003) 22:3568–79. doi: 10.1093/emboj/cdg355

PubMed Abstract | CrossRef Full Text | Google Scholar

34. Monserrate JP, Chen MY, Brachmann CB. Drosophila larvae lacking the bcl-2 gene, buffy, are sensitive to nutrient stress, maintain increased basal target of rapamycin (Tor) signaling and exhibit characteristics of altered basal energy metabolism. BMC Biol. (2012) 10:63. doi: 10.1186/1741-7007-10-63

PubMed Abstract | CrossRef Full Text | Google Scholar

35. Bjorkqvist M, Wild EJ, Thiele J, Silvestroni A, Andre R, Lahiri N, et al. A novel pathogenic pathway of immune activation detectable before clinical onset in Huntington's disease. J Exp Med. (2008) 205:1869–77. doi: 10.1084/jem.20080178

PubMed Abstract | CrossRef Full Text | Google Scholar

36. Trager U, Andre R, Lahiri N, Magnusson-Lind A, Weiss A, Grueninger S, et al. HTT-lowering reverses Huntington's disease immune dysfunction caused by NFkappaB pathway dysregulation. Brain. (2014) 137:819–33. doi: 10.1093/brain/awt355

PubMed Abstract | CrossRef Full Text | Google Scholar

37. Lemaitre B, Hoffmann J. The host defense of Drosophila melanogaster. Annu Rev Immunol. (2007) 25:697–743. doi: 10.1146/annurev.immunol.25.022106.141615

PubMed Abstract | CrossRef Full Text | Google Scholar

38. Basset A, Khush RS, Braun A, Gardan L, Boccard F, Hoffmann JA, et al. The phytopathogenic bacteria Erwinia carotovora infects Drosophila and activates an immune response. Proc Natl Acad Sci USA. (2000) 97:3376–81. doi: 10.1073/pnas.97.7.3376

PubMed Abstract | CrossRef Full Text | Google Scholar

39. Wild E, Magnusson A, Lahiri N, Krus U, Orth M, Tabrizi SJ, et al. Abnormal peripheral chemokine profile in Huntington's disease. PLoS Curr. (2011) 3:Rrn1231. doi: 10.1371/currents.RRN1231

PubMed Abstract | CrossRef Full Text | Google Scholar

40. Chen CM, Wu YR, Cheng ML, Liu JL, Lee YM, Lee PW, et al. Increased oxidative damage and mitochondrial abnormalities in the peripheral blood of Huntington's disease patients. Biochem Biophys Res Commun. (2007) 359:335–40. doi: 10.1016/j.bbrc.2007.05.093

PubMed Abstract | CrossRef Full Text | Google Scholar

41. Zwilling D, Huang SY, Sathyasaikumar KV, Notarangelo FM, Guidetti P, Wu HQ, et al. Kynurenine 3-monooxygenase inhibition in blood ameliorates neurodegeneration. Cell. (2011) 145:863–74. doi: 10.1016/j.cell.2011.05.020

PubMed Abstract | CrossRef Full Text | Google Scholar

42. Bouchard J, Truong J, Bouchard K, Dunkelberger D, Desrayaud S, Moussaoui S, et al. Cannabinoid receptor 2 signaling in peripheral immune cells modulates disease onset and severity in mouse models of Huntington's disease. J Neurosci. (2012) 32:18259–68. doi: 10.1523/JNEUROSCI.4008-12.2012

PubMed Abstract | CrossRef Full Text | Google Scholar

43. Sawa A, Wiegand GW, Cooper J, Margolis RL, Sharp AH, Lawler JF Jr, et al. Increased apoptosis of Huntington disease lymphoblasts associated with repeat length-dependent mitochondrial depolarization. Nat Med. (1999) 5:1194–8. doi: 10.1038/13518

PubMed Abstract | CrossRef Full Text | Google Scholar

44. Anderl I, Vesala L, Ihalainen TO, Vanha-Aho LM, Ando I, Ramet M, et al. Transdifferentiation and proliferation in two distinct hemocyte lineages in Drosophila melanogaster larvae after wasp infection. PLoS Pathog. (2016) 12:e1005746. doi: 10.1371/journal.ppat.1005746

PubMed Abstract | CrossRef Full Text | Google Scholar

45. Keebaugh ES, Schlenke TA. Insights from natural host-parasite interactions: the Drosophila model. Dev Comp Immunol. (2014) 42:111–23. doi: 10.1016/j.dci.2013.06.001

PubMed Abstract | CrossRef Full Text | Google Scholar

46. Fauvarque MO, Williams MJ. Drosophila cellular immunity: a story of migration and adhesion. J Cell Sci. (2011) 124:1373–82. doi: 10.1242/jcs.064592

PubMed Abstract | CrossRef Full Text | Google Scholar

47. Castillo JC, Shokal U, Eleftherianos I. Immune gene transcription in Drosophila adult flies infected by entomopathogenic nematodes and their mutualistic bacteria. J Insect Physiol. (2013) 59:179–85. doi: 10.1016/j.jinsphys.2012.08.003

PubMed Abstract | CrossRef Full Text | Google Scholar

48. Trager U, Andre R, Magnusson-Lind A, Miller JR, Connolly C, Weiss A, et al. Characterisation of immune cell function in fragment and full-length Huntington's disease mouse models. Neurobiol Dis. (2015) 73:388–98. doi: 10.1016/j.nbd.2014.10.012

PubMed Abstract | CrossRef Full Text | Google Scholar

49. Swanson JA. Shaping cups into phagosomes and macropinosomes. Nat Rev Mol Cell Biol. (2008) 9:639–49. doi: 10.1038/nrm2447

PubMed Abstract | CrossRef Full Text | Google Scholar

50. Morin-Poulard I, Vincent A, Crozatier M. The Drosophila JAK-STAT pathway in blood cell formation and immunity. JAKSTAT. (2013) 2:e25700. doi: 10.4161/jkst.25700

PubMed Abstract | CrossRef Full Text | Google Scholar

51. Wang G. Human antimicrobial peptides and proteins. Pharmaceuticals. (2014) 7:545–94. doi: 10.3390/ph7050545

PubMed Abstract | CrossRef Full Text | Google Scholar

52. Anderson AN, Roncaroli F, Hodges A, Deprez M, Turkheimer FE. Chromosomal profiles of gene expression in Huntington's disease. Brain. (2008) 131:381–8. doi: 10.1093/brain/awm312

PubMed Abstract | CrossRef Full Text | Google Scholar

53. Lin DM, Goodman CS. Ectopic and increased expression of Fasciclin II alters motoneuron growth cone guidance. Neuron. (1994) 13:507–23. doi: 10.1016/0896-6273(94)90022-1

PubMed Abstract | CrossRef Full Text | Google Scholar

54. Sinenko SA, Mathey-Prevot B. Increased expression of Drosophila tetraspanin, Tsp68C, suppresses the abnormal proliferation of ytr-deficient and Ras/Raf-activated hemocytes. Oncogene. (2004) 23:9120–8. doi: 10.1038/sj.onc.1208156

PubMed Abstract | CrossRef Full Text | Google Scholar

55. Zettervall CJ, Anderl I, Williams MJ, Palmer R, Kurucz E, Ando I, et al. A directed screen for genes involved in Drosophila blood cell activation. Proc Natl Acad Sci USA. (2004) 101:14192–7. doi: 10.1073/pnas.0403789101

PubMed Abstract | CrossRef Full Text | Google Scholar

56. Zhou L, Schnitzler A, Agapite J, Schwartz LM, Steller H, Nambu JR. Cooperative functions of the reaper and head involution defective genes in the programmed cell death of Drosophila central nervous system midline cells. Proc Natl Acad Sci USA. (1997) 94:5131–6. doi: 10.1073/pnas.94.10.5131

PubMed Abstract | CrossRef Full Text | Google Scholar

57. Warrick JM, Paulson HL, Gray-Board GL, Bui QT, Fischbeck KH, Pittman RN, et al. Expanded polyglutamine protein forms nuclear inclusions and causes neural degeneration in Drosophila. Cell. (1998) 93:939–49. doi: 10.1016/S0092-8674(00)81200-3

PubMed Abstract | CrossRef Full Text | Google Scholar

58. Ibrahim E, Dobes P, Kunc M, Hyrsl P, Kodrik D. Adipokinetic hormone and adenosine interfere with nematobacterial infection and locomotion in Drosophila melanogaster. J Insect Physiol. (2018) 107:167–74. doi: 10.1016/j.jinsphys.2018.04.002

PubMed Abstract | CrossRef Full Text | Google Scholar

59. Zhang S, Binari R, Zhou R, Perrimon N. A genomewide RNA interference screen for modifiers of aggregates formation by mutant Huntingtin in Drosophila. Genetics. (2010) 184:1165–79. doi: 10.1534/genetics.109.112516

PubMed Abstract | CrossRef Full Text | Google Scholar

60. Han SK, Lee D, Lee H, Kim D, Son HG, Yang JS, et al. OASIS 2: online application for survival analysis 2 with features for the analysis of maximal lifespan and healthspan in aging research. Oncotarget. (2016) 7:56147–52. doi: 10.18632/oncotarget.11269

PubMed Abstract | CrossRef Full Text | Google Scholar