Chagas disease is caused by infection with the protozoan Trypanosoma cruzi (T. cruzi) and is an important cause of severe inflammatory heart disease. However, the mechanisms driving Chagas disease cardiomyopathy have not been completely elucidated. Here, we show that the canonical PI3Kγ pathway is upregulated in both human chagasic hearts and hearts of acutely infected mice. PI3Kγ-deficient mice and mutant mice carrying catalytically inactive PI3Kγ are more susceptible to T. cruzi infection. The canonical PI3Kγ signaling in myeloid cells is essential to restrict T. cruzi heart parasitism and ultimately to avoid myocarditis, heart damage, and death of mice. Furthermore, high PIK3CG expression correlates with low parasitism in human Chagas’ hearts. In conclusion, these results indicate an essential role of the canonical PI3Kγ signaling pathway in the control of T. cruzi infection, providing further insight into the molecular mechanisms involved in the pathophysiology of chagasic heart disease.
Chagas disease is caused by infection with the intracellular protozoan parasite Trypanosoma cruzi (T. cruzi). Currently, approximately 6–7 million people worldwide, mostly in Latin America, are infected1,2. At present, due to migration to North America, Europe, and Japan, it is a global health concern3,4,5,6. The disease is characterized by an acute phase, usually asymptomatic and with evident parasitemia detectable in the bloodstream7. In most individuals, manifestations of the acute phase disappear a few weeks after infection8, followed by the chronic phase of infection. Although the chronic phase of Chagas disease is most likely featured by the asymptomatic form, approximately 30% of patients develop the cardiac form9. Life-threatening chronic chagasic cardiomyopathy (CCC) is the most severe manifestation of the disease, which is characterized by an intense Th1 T-cell and macrophage-rich myocarditis, destruction of myofibers, and alteration of cardiac function10,11. It can lead to refractory heart failure and sudden death in a significant proportion of patients. The molecular mechanisms involved in the pathophysiology of chagasic heart disease are unclear.
Recognition of the parasite by resident and recruited leukocytes activates several signaling pathways, including phosphatidylinositol 3-kinases (PI3Ks) signaling, which is involved in different cellular processes through the phosphorylation of lipids and proteins12,13. Among the PI3K enzyme family, PI3Kγ signaling is activated by the βγ subunit of G-protein-coupled receptors and plays an important role in leukocyte functions, inflammation, and heart dysfunction14.
Here, we show that the canonical PI3Kγ is involved in the pathophysiology of chagasic heart disease. The canonical PI3Kγ pathway is upregulated in both human chagasic hearts and hearts of acutely infected mice. Deficient mice in the canonical PI3Kγ signaling are more susceptible to T. cruzi infection. The canonical PI3Kγ signaling in myeloid cells restricts heart parasitism and avoids heart damage and death of mice. Furthermore, high PIK3CG expression correlates with low parasitism in human chagasic hearts. These data identify a previously unrecognized role of the canonical PI3Kγ signaling pathway in the control of T. cruzi infection, providing further insight into the molecular mechanisms involved in chagasic heart disease.
Canonical PI3Kγ signaling protects from T. cruzi infection
We initially examined the expression and activation of PI3Kγ signaling in the heart tissue of T. cruzi-infected mice. For this purpose, we performed analysis of the cardiac tissue transcriptome from T. cruzi Y strain-infected C57BL/6 mice previously obtained by our group15 (GSE41089). Data revealed that the expression of Pik3cg (P = 4.0E-3; unpaired t-test) and Pik3cd (P = 7.4E-6; unpaired t-test) genes, but not Pik3ca, are upregulated in the heart tissue of T. cruzi-infected mice 18 days post infection (dpi) (Fig. 1a). Corroborating our transcriptome analysis, heart tissue of infected C57BL/6 mice showed an increased mRNA expression of Pik3cg and Pik3cd genes, but not Pik3ca, compared to heart samples from uninfected mice (Fig. 1b). Following activation, PI3Kγ promotes downstream signaling through the protein kinase B (AKT) pathway16. The phosphorylated forms of AKT (pAKT) were thus studied as markers of the canonical PI3Kγ signaling activation. AKT is a family of kinases consisting of three isoforms of AKTs, AKT1, AKT2, and AKT3 encoded by independent genes. AKT1 and AKT2 are expressed in leukocytes and have been implicated in the immune response17. In this context, we sought to investigate whether PI3Kγ signaling was enhanced in the heart tissue of T. cruzi-infected mice through the measurement of pAKTs (pAKT1 and pAKT2). Although the infection does not change the expression levels of Akt1 and Akt2 mRNA (Supplementary Fig. 1a, b) and proteins (Fig. 1c, d), the phosphorylated forms of these proteins are upregulated in the heart tissue of infected mice compared to the uninfected group (Fig. 1c, d). These results indicate that after infection with T. cruzi, PI3Kγ signaling is upregulated in the heart of infected mice.
To evaluate whether PI3Kγ signaling pathways contribute for the pathogenesis of chagasic disease, we took advantage of the experimental mouse model of this disease. In this context, wild-type (WT) and Pik3cg−/− mice were infected with T. cruzi Y strain. Unlike C57BL/6 WT mice, which had a slight reduction in their body weight during infection, Pik3cg−/− mice presented a significant reduction in their body weight starting at 9th day after infection and progressively worsened (Fig. 2a). Moreover, differently of the WT-infected mice, which presented 100% of survival, all the infected Pik3cg−/− mice succumbed until 30 dpi (Fig. 2b). Remarkably, heterozygous Pik3cg+/− mice were protected from death caused by T. cruzi infection when compared with homozygous Pik3cg−/− mice (Supplementary Fig. 2). Although biological activities of PI3Kγ have been ascribed mainly by its ability to convert PIP2 into PIP3, there is also evidence that PI3Kγ can act as a scaffold protein, independently of the kinase function18. In this context, we infected mutant mice carrying a catalytically inactive PI3Kγ (Pik3cgKD/KD)18. Similarly to Pik3cg−/− mice, Pik3cgKD/KD mice were also susceptible to T. cruzi infection (Fig. 2c). In agreement with genetic inhibition of the PI3Kγ catalytic activity, pharmacological inhibition of PI3Kγ activity in WT mice with a partial selective PI3Kγ isoform inhibitor, AS605240, increased the weight loss and mortality when compared to vehicle-treated mice (Supplementary Fig. 3a, b). Despite of having a high mortality rate, Pik3cg−/− and Pik3cgKD/KD mice showed similar numbers of circulating parasites in the blood across the whole time course compared to WT mice (Fig. 2d, e), suggesting that the inefficient control of the systemic parasitemia is not the cause of the increased Pik3cg−/− and Pik3cgKD/KD mice mortality. To evaluate in which cell type (cardiomyocytes or hematopoietic cells/leukocytes) PI3Kγ signaling is important for the pathophysiology of chagasic heart disease, bone marrow (BM) chimeric mice were generated. Interestingly, the transfer of BM from WT mice to irradiated Pik3cg−/− mice protected recipient mice from T. cruzi infection-induced death (Fig. 2f). These data suggest that an integral PI3Kγ signaling pathway in hematopoietic cells/leukocytes is central for the control of T. cruzi infection.
PI3Kγ protects from T. cruzi infection-induced cardiac damage
To elucidate the cause of the increased susceptibility to T. cruzi infection by Pik3cg−/− mice, we analyzed whether these animals developed heart complications. The heart damage was quantified by serum CK-MB activity, an enzyme located in the cytosol of the cardiomyocytes that is released into the blood after heart damage19. The activity of CK-MB was significantly increased in T. cruzi-infected Pik3cg−/− mice compared with its activity in WT mice (Fig. 3a), indicating an enhancement of the heart damage in Pik3cg−/− mice. Pik3cgKD/KD mice also showed high levels of serum CK-MB after T. cruzi infection (Fig. 3b). Further supporting heart dysfunction in Pik3cg−/− mice after infection, echocardiography revealed a concentric hypertrophy, along with a clear reduction in left ventricle diameter and cardiac output and no reduction in ejection fraction (Fig. 3c–g). These findings are indicative of a pathological adaptation of the heart leading to heart failure with preserved left ventricular ejection fraction20,21. Overall, the preceding data suggest that the canonical PI3Kγ signaling pathway protects mice from T. cruzi infection-induced heart damage and dysfunction.
Chagasic myocarditis is enhanced in PI3Kγ-deficient mice
To further understand why the canonical PI3Kγ signaling pathway protects mice from T. cruzi-induced heart damage and dysfunction, we next analyzed heart myocarditis in these mice. Although PI3Kγ signaling is very important for leukocyte migration in several models of inflammation22,23,24,25, histopathological analysis of the heart tissue from T. cruzi-infected Pik3cg−/− mice revealed an increase in leukocytes infiltration in comparison to WT mice (Fig. 4a). In agreement with this finding, multiplex analyses of cytokines/chemokines profile in the heart tissue of Pik3cg−/− (Fig. 4b and Supplementary Table 1) and Pik3cgKD/KD (Supplementary Fig. 4 and Supplementary Table 2) mice revealed an increase in the levels of pro-inflammatory cytokines (e.g., TNF, IFN-γ, and IL-6), and chemokines (e.g., RANTES, MCP-1, and MIP-1α), whereas anti-inflammatory cytokines are downregulated (e.g., IL-10 and IL-13) when compared to infected WT mice. At the same period of infection, the production of pro-inflammatory and anti-inflammatory cytokines in the blood and spleen was not different between WT and Pik3cg−/− mice (Supplementary Fig. 5), suggesting that the PI3Kγ signaling modulates inflammatory response in T. cruzi infection is specific for the heart tissue. Supporting the enhanced myocarditis, the number of CD4+ T-cells infiltrating the heart tissue of Pik3cg−/−-infected mice was increased compared to WT mice (Fig. 4c). Consistent with human chagasic cardiomyopathy26, the real-time qPCR analysis in the heart revealed that CD4+ T-cells mainly express the mRNA of the Th1-related transcription factor Tbet, compared with Th2 (Gata3) and Th17 (Rorgt) cells (Fig. 4d). In the absence of PI3Kγ, Tbet expression was increased compared to WT controls (Fig. 4d). In addition, post treatment of Pik3cg−/−-infected mice with a low dose of dexamethasone (glucocorticoid) reversed their susceptibility to T. cruzi infection (Fig. 4e). Collectively, these results indicate that enhanced myocarditis of infected Pik3cg−/− and Pik3cgKD/KD mice might explain enhanced heart dysfunction and mortality.
Since PI3Kγ signaling appears to controls the production of inflammatory mediators after infection with T. cruzi, we investigated whether this effect might be related to the number and suppressive function of regulatory T-cells. It was found that the number of CD4+ Foxp3+ regulatory T-cells (Tregs) was not different in the heart tissue of Pik3cg−/− and WT mice at 18 dpi (Fig. 5a). Furthermore, the expression of the regulatory markers in Tregs from infected heart of WT and Pik3cg−/−, Foxp3 (Fig. 5b, c), CTLA-4 (Fig. 5d), and CD39 (Fig. 5e) were also similar. In addition, the PI3Kγ deficiency did not interfere with the suppressor function of Tregs (CD4+ CD25+) cells isolated from lymph nodes of naive mice (Fig. 5f). These results ruled out that a disturbance in Tregs cells might explain the enhanced chagasic myocarditis of Pik3cg−/− mice compared to WT controls.
PI3Kγ signaling in myeloid cells reduces T. cruzi infection
Because PI3Kγ signaling deficiency leads to a large number of inflammatory cells and higher levels of inflammatory mediators in the heart tissue of infected mice, we evaluated whether these cells were able to control heart parasitism. Of note, an increased number of amastigote nests were detected in the heart of Pik3cg−/− mice when compared to WT mice (Fig. 6a). According to the histological findings, the heart tissue of infected Pik3cg−/− or Pik3cgKD/KD mice showed increased amount of parasite DNA compared to infected WT mice (Fig. 6b, c). Supporting the hypothesis that Pik3cg−/− mice died due to uncontrolled heart infection, post treatment (after parasitemia has falling down) with benznidazole, the standard trypanocidal drug used for T. cruzi infection27, protected Pik3cg−/− mice from death when compared to vehicle-treated mice (Fig. 6d).
Heart T. cruzi parasitism control is orchestrated mainly by infiltrating CD8+ T-cells and activated macrophages28,29,30,31. Thus, we evaluated the presence and function of these cells to elucidate the mechanisms of uncontrolled heart parasitism in Pik3cg−/− mice. Numbers of infiltrating CD8+ T-cells in the heart of Pik3cg−/−-infected mice did not differ from WT mice (Supplementary Fig. 6a). In addition, the in vivo cytotoxic activity of CD8+ T-cells in infected Pik3cg−/− mice was similar to WT mice (Supplementary Fig. 6b), indicating that a defect in CD8+ T-cells was not responsible for the Pik3cg−/− mice susceptibility to control heart parasitism.
To further investigate why Pik3cg−/− mice failed to control cardiac parasitism, we next determined whether a dysfunction in migration and/or function of myeloid cells (e.g., macrophages) could be involved. First, recruitment of CD11b+ cells into the heart of infected Pik3cg−/− mice was similar to infected WT mice (Fig. 7a). However, CD11b+ cells isolated from the heart of Pik3cg−/− or Pik3cgKD/KD mice exhibited higher parasite levels compared with CD11b+ cells isolated from WT mice (Fig. 7b). Although the parasitism in CD11b− cells from Pik3cg−/− and Pik3cgKD/KD mice was also higher, intracellular parasite levels were lower than in CD11b+ cells (Fig. 7b). To further understand the mechanisms by which Pik3cg−/−-deficient myeloid cells failed to control intracellular T. cruzi infection, we investigated the ability of bone marrow-derived macrophages (BMDMs) from Pik3cg−/− mice to control the intracellular T. cruzi in vitro.
Corroborating the in vivo findings, BMDMs from Pik3cg−/− mice treated with IFN-γ were remarkably less effective in killing the parasite than WT BMDMs (Fig. 7c). In addition, the number of trypomastigote forms released into the supernatant from the Pik3cg−/− BMDM culture was higher than in supernatant from the WT BMDM culture (Fig. 7d). The increase in the nitric oxide (NO) production by macrophages is the most important mechanism involved in their microbicidal activity against T. cruzi32,33. In association with the impaired ability to kill intracellular T. cruzi, infected Pik3cg−/− BMDMs produced lower amounts of NO compared to infected WT BMDMs (Fig. 7e). We then proceeded to investigate whether the heart macrophages from Pik3cg−/− mice had a reduced parasite-killing capacity because they were not able to produce NO in vivo. PI3Kγ was found to be essential for NO production in the heart of T. cruzi-infected mice since the concentration of nitrate in the infected heart tissue was reduced in Pik3cg−/− mice as compared with the WT group (Fig. 7f). Then, we investigated whether PI3Kγ signaling was also important for the microbicidal function of human macrophages against T. cruzi infection in vitro. Corroborating the mouse data, pharmacological inhibition of PI3Kγ reduced the ability of human macrophages (THP-1) to kill intracellular parasites (Fig. 7g).
Finally, to validate that the canonical PI3Kγ signaling in myeloid cells was important to counteract heart parasitism and confer resistance to infection in vivo, mice harboring a conditional deletion of AKT1 in LysM+ cells (Akt1−/−Lysmcre) were used34. Of note, Akt1−/−Lysmcre mice were more susceptible to T. cruzi infection when compared to control littermates (Fig. 8a). In agreement, heart parasitism was not controlled in Akt1−/−Lysmcre mice (Fig. 8b). Conversely, Akt2−/− mice were as resistant to T. cruzi infection as WT mice (Fig. 8c), indicating that AKT1, but not AKT2, was involved in the downstream events of PI3Kγ signaling responsible for the control of T. cruzi infection. Taken together, these results indicated that a canonical PI3Kγ/AKT1 signaling deficiency in myeloid cells led to an inability to control heart T. cruzi infection and ultimately avoid heart damage and host death.
PI3Kγ signaling in human chagasic myocarditis
To translate our findings in the mouse model to the human disease, we examined the expression and activation of PI3Kγ signaling in the heart samples of chagasic disease patients. Human heart tissue transcriptome (GSE84796) revealed that the expression of PIK3CG gene was upregulated in the samples from patients with CCC when compared to heart samples from healthy control individuals (Ctl) (relative expression = 5.37; P = 1.0E-5; Student’s t-test with the Benjamini–Hochberg method) or even samples from patients with non-chagasic cardiomyopathy (idiopathic dilated cardiomyopathy, DCM, GSE111544, Relative expression = 6.60; P = 2.1E-8; Student’s t-test with the Benjamini–Hochberg method) (Fig. 9a). None of the other members of the class 1 PI3K family (α, β, and δ subunits) appeared to be modulated as dramatically as the PIK3CG gene (Fig. 9a). To validate the transcriptome data, samples from human hearts were used for the evaluation of PIK3CG expression by real-time PCR. Corroborating our transcriptome analyses, PIK3CG and PIK3CD expression were upregulated (Fig. 9b), whereas the expression of PIK3CA and PIK3CB was similar in the heart samples from CCC patients in comparison to those from healthy control individuals or DCM patients (Fig. 9b). Next, we verified the activation of PI3Kγ signaling in the chagasic human samples. Although there was no change in AKT1 and AKT2 mRNA (GSE84796 and validation—Supplementary Fig. 1c, d) and protein expression (Fig. 9c, d), the activated forms of AKT1 and AKT2 (pAKT1 and pAKT2) were increased in the heart tissue from CCC patients compared to those from DCM patients or healthy controls (Fig. 9c, d). To analyze the interactions between PI3Kγ and the heart immune response, a correlation analysis was performed using the transcriptome data set from CCC patients (GSE84796). The expression of the PIK3CG gene positively correlated with the expression of myeloid cells markers (CD11b, CD300a, and CD33) and inflammatory mediators genes (Supplementary Fig. 7a–h), indicating that the increased influx of leukocytes in chagasic hearts might be the cause of the increase in PI3Kγ expression. To validate these findings, real-time PCR was performed in the heart samples. The expression of pro-inflammatory cytokines (TNF and IFNG) and chemokines (CCL5/RANTES) was higher in heart tissue of CCC patients compared with the DCM or control groups (Supplementary Fig. 8a–c). In agreement, there was a positive correlation in heart tissue of CCC patients between the expression of the PIK3CG gene and the proinflammatory genes TNF (r2 = 0.42; P = 0.16, Pearson’s test), IFNG (r2 = 0.62; P = 0.061, Pearson’s test), and CCL5/RANTES (r2 = 0.68; P = 0.042, Pearson’s test) (Supplementary Fig. 8d–f).
Finally, we also analyzed the interaction between PI3Kγ expression and heart parasitism to validate the hypothesis that PI3Kγ participates in the mechanisms that control heart T. cruzi infection. Real-time PCR analyses of T. cruzi DNA in the heart samples of CCC patients revealed two distinct groups of patients regarding the levels of parasitism. Some of them had low levels of heart parasitism, which were almost undetectable, and others showed significant parasitism (Fig. 10a). When we stratified these two groups, we found that the expression of PIK3CG was much higher in the group with low parasitism (Fig. 10b). Collectively, these results indicated that similarly the findings obtained in the mouse model of T. cruzi infection, PI3Kγ signaling was also upregulated in the heart tissue of one group of chagasic disease patients and that this signaling might also be acting as a counteracting mechanism of heart T. cruzi parasitism.
Characterization of the pathophysiological aspects of heart T. cruzi infection and the mechanisms that lead to resistance or susceptibility of the host is fundamental to understand the Chagas disease and to propose novel targets to prevent the development of the severe form of this disease. In this regard, identification of the intracellular signaling pathways activated in response to T. cruzi infection is critical. In the present study, we investigated the role of PI3Kγ signaling in the heart of T. cruzi-infected mice and humans. Our findings indicate that canonical PI3Kγ/AKT1 signaling is upregulated in the heart tissue of T. cruzi-infected mice and humans with the Chagas disease. Finally, we further demonstrated an essential role of the canonical PI3Kγ signaling in myeloid cells (e.g., macrophages) to restrict heart parasitism and consequently avoid heart inflammation/damage and dysfunction.
The activation of PI3K signaling has been demonstrated during in vitro infections of human and mouse macrophages with T. cruzi35,36,37. To our knowledge, this is the first study to provide further evidence that canonical PI3Kγ signaling, together with its downstream pathway AKT1, is activated in the heart tissue from chagasic patients and mice infected with T cruzi. Herein, we found that in the absence of canonical PI3Kγ signaling in hematopoietic cells, mice are highly susceptible to T. cruzi infection, which is associated with an uncontrolled heart parasitism and exacerbated inflammatory response. Since PI3Kγ pathway is activated by GPCRs, such as chemokine receptors, this signaling is crucial for leukocyte migration, genetic or pharmacological inhibition of this kinase decreases the inflammation and ameliorates the score in several models of inflammatory diseases22,23,24,38. Our data showed that the ablation of PI3Kγ does not inhibit the T. cruzi-induced leukocyte migration to the heart tissue, suggesting that during T cruzi infection, leukocyte migration is not mediated by canonical PI3Kγ signaling, and other chemotaxis signaling events might play a role during the infection.
It is established that PI3Kγ signaling also plays an important role in cardiomyocytes physiology and that its absence can aggravate some cardiomyopathies18,39. Our data indicate that the participation of PI3Kγ signaling in the pathophysiology of chagasic heart disease seems to be more related to its function in heart-infiltrating myeloid cells. This result is apparently different from the evidence showing that during the chronic phase of T. cruzi infection, the PI3K/AKT/NO axis in cardiomyocytes contributes to the development of electric dysfunction of cardiomiocytes40. Nevertheless, these differences could be explained by the different stage of the disease or even by different PI3K isoform involved40. Furthermore, the impact of the PI3K/AKT/NO pathway in cardiomyocytes on the in vivo outcome has been not evaluated40.
Chagasic heart failure has been attributed to increased levels of local or systemic pro-inflammatory cytokines/chemokines27. In addition to the inability to restrict the heart parasitism, our data showed an enhanced production of pro-inflammatory cytokines and chemokines in the cardiac tissue of Pik3cg−/− mice. Although this “cytokine storm” might be merely a consequence of uncontrolled parasitism, it seems strictly important for the increased susceptibility. This hypothesis was supported by the findings that treatment with a low dose of glucocorticoid is able to reverse Pik3cg−/− mouse susceptibility. Nevertheless, we cannot eliminate the possibility that PI3Kγ signaling pathway directly dampen the inflammatory response in the heart of infected mice. In fact, a recent study has demonstrated that the activation of PI3Kγ signaling counteracts inflammatory cytokines and chemokines production by macrophages41.
The finding that canonical PI3Kγ signaling is also increased in the heart tissue of CCC patients is consistent with the observed tissue leukocyte infiltration. Furthermore, our finding that patients with lower heart parasitism have higher cardiac expression of PI3Kγ supports our hypothesis that this kinase contributes to the containment of T. cruzi infection. On the other hand, some patients develop CCC despite having high expression/activation of canonical PI3Kγ signaling and controlling the parasitism in the heart. Nevertheless, as myocarditis is the prime process of CCC progression42, partial control of heart parasitism due to PI3Kγ-expressing myeloid cells occurs at the expense of tissue-damaging inflammation, likely leading to myocarditis and the development of cardiomyopathy in such chronically infected individuals. Consistently, we propose that PI3Kγ signaling might be a protective mechanism that restricts heart parasitism to avoid a rapid progression of the disease, which usually takes several years to chronify. Finally, we hypothesize that alterations that change PI3Kγ expression and/or function (due to polymorphisms, mutations) could be a factor involved in the susceptibility of some patients to developing cardiac forms of Chagas disease. Further studies are necessary to test this hypothesis.
Collectively, the present study has demonstrated the crucial role of the canonical PI3Kγ signaling for host resistance to T. cruzi infection. Furthermore, the canonical PI3Kγ signaling in heart-infiltrating myeloid cells is crucial for optimal microbicidal activity that leads to the control of heart parasitism and to the avoidance of exacerbated myocarditis and heart damage. In conclusion, we believe that our data provided further insight into the molecular mechanisms of the pathophysiology of chagasic heart disease.
Female C57BL/6 WT, PI3Kγ-deficient mice (Pik3cg−/−)43, and PI3Kγ kinase dead mutant mice (Pik3cgKD/KD)44 aged 6–8 weeks were bred and maintained at the animal facility of the Ribeirão Preto Medical School University of São Paulo, Ribeirão Preto, Brazil. Female conditional Akt1−/−Lysmcre were generated by crossing Akt1fl/fl mice34 (kindly provided by Prof. P. Tsichlis, Tufts University, Boston, USA) and Lysmcre mice (Jackson Laboratories). Akt1−/−Lysmcre mice, littermate controls and Akt2−/− mice45 (kindly provided by Prof. M. Birnbaum, U. Pennsylvania, Philadelphia, USA) were maintained at the animal facility of the Medical School, University of Crete and IMBB-FORTH, Greece. Pik3cg+/− mice were generated by crossing Pik3cg−/− mice with C57BL/6 WT mice. The animals were maintained in micro-isolator cages under standard conditions and fed with food and water ad libitum. The Institutional Ethics Committee in Animal Experimentation—CEUA of the Ribeirão Preto Medical School, University of São Paulo (Protocol number 196/2009) and the Veterinary Department of the Crete Region, Medical School, University of Crete and IMBB-FORTH, Heraklion, Crete, Greece (Protocol number 27298/2014) approved the experimental protocols. Mice were selected based on their genotype. All other criteria were not considered and as such, randomized. We were not blinded to the mouse genotypes or group allocations except where mentioned.
All experiments were conducted using trypomastigote forms of human isolated T. cruzi Y strain46. For in vitro experiments, parasites were grown for 7–9 days in a fibroblast cell line LLC-MK2 (American Type Culture Collection-ATCC®, cat. CCL-7™) and suspended in RPMI 1640 medium (Gibco-BRL Life Technologies, Grand Island, NY, USA). For in vivo experiments, mice were inoculated intraperitoneally with 103 bloodstream trypomastigote forms. From day 5 after infection, blood parasitemia was evaluated in 5 μl of blood from the tail vein by counting 100 fields through direct observation under an optical microscope. Additionally, the body weight of the mice was also measured. The survival rate was assessed daily. Infected animals were excluded (pre-established) from the study when parasitemia was not detected at day 9 post infection.
Real-time quantitative PCR
For RT-PCR, total RNA was isolated form heart samples with TRIzol using the specific kit RNeasy mini kit (Qiagen), and cDNA was synthesized with the ThermoScript RT-PCR system (Invitrogen). PCR was carried with StepOnePlus (Applied Biosystems) using SYBR Green GoTaq qPCR MasterMix (Promega). The endogenous control Gapdh was used to normalize gene expression. The sequences of the primers are shown in Supplementary Table 3.
Western blot analysis
Protein lysates from human or mouse heart samples were prepared in RIPA buffer supplemented with a cocktail of protease and phosphatase inhibitors (Cell Signaling). Equal amounts of total proteins were loaded and separated in SDS-polyacrylamide gel. After electrophoresis, the proteins were electrotransferred onto nitrocellulose membranes (0.2 μm, GE Healthcare) and incubated for 1 h with 5% bovine serum albumin followed by overnight incubation at 4 °C with primary antibody. Finally, the membranes were incubated for 1 h with secondary antibodies conjugated to horseradish peroxidase. Immunoblots were visualized with the Western Blotting Chemiluminescence Luminol (Pierce, Thermo Fisher Scientific Inc.) using the ChemiDoc™ XRS System (Bio-Rad). The primary antibodies used in the study were: phospho-AKT1 (1:600; Cell Signaling, cat. 9018); total AKT1 (1:1000; Cell Signaling, cat. 2938); phospho AKT2 (1:600, Cell Signaling, cat. 8599); total AKT2 (1:1000; Cell Signaling, cat. 3063); and GAPDH (1: 5000; Sigma-Aldrich, cat. G9545). Full scans of the original uncropped western blots are shown in Supplementary Figs. 9 and 10.
Serum CK-MB activity assay
To evaluate cardiac damage, the activity of CK-MB was measured in the sera of mice infected with T. cruzi. Quantification was performed using a kinetic method with specific kit CK-MB Liquiform (Labtest®) followed by read in spectrophotometer at 340 nm (EMAX Molecular Devices Corporation®).
Mice were anesthetized with 1.5% isofluorane (Forane® Isoflurane, USP) in an inhalation chamber. Body temperature was monitored, and cardiac parameters were obtained through VEVO2100® machine using a 30 MHz transducer. Diastolic left ventricle diameter and ventricular posterior wall thickness were evaluated in M mode; ejection fraction and cardiac output were calculated in bidimensional mode.
Heart samples were fixed in 10% buffered formalin solution and, after 72 h, dehydrated in a crescent concentration of ethanol solutions and embedded in paraffin. Blocks were sectioned at thickness of 5 μm and stained with haematoxylin-eosin (H&E). Using a light microscope, the number of amastigote nests was counted in 25 images of each animal of the group, the inflammation was estimated with ImageTool 2.0 software (University of Texas Health Science Center, TX, USA). The pathologist who performed the histological analysis was blinded to the mice genotypes.
Treatment with PI3Kγ inhibitor
WT mice were divided in two groups and treated subcutaneously with 30 mg kg− of PI3Kγ inhibitor AS605240 (5-Quinoxalin-6-ylmethylene-thiazolidine-2,4-dione—Alexis®) or vehicle (2% DMSO)47. Mice were treated once a day starting from the peak of parasitemia (day 9 of infection) for 10 days.
Cytokines and chemokines measurement
Measurement of cytokines and chemokines in the heart tissue of mice was performed by Milliplex® (Merck Millipore) assay in accordance with the manufacturer’s instructions.
Production of the cytokines IFN-γ, TNF-α, IL-10, and IL-4 (R&D Systems, Minneapolis, MN) was assessed in the serum and spleen of WT and Pik3cg−/− naive mice or 18 days after infection with 103 trypomastigote forms of T. cruzi Y strain. Fragments of spleen were collected into vials with a protease inhibitor cocktail (Complete, Roche), macerated, and centrifuged, and the supernatant collected for cytokine quantification. Measurements were performed through by ELISA assay, using specific kit (DuoSet®, R&D Systems) according to manufacturer’s instructions.
The mouse heart tissue was sliced into small pieces and digested using Liberase TL (Roche) for 1 h at 37 °C/5% CO2. The obtained cells suspension was filtered through a 40 µm cell strainer (Corning®), and isolated cells were counted in a Neubauer chamber and then incubated with specific antibodies. The following antibodies were used: APC-Cy7 rat anti-mouse CD45 (1: 200, clone 30-F11, BD Biosciences, cat. 557659); FITC armenian hamster anti-mouse CD3 (1:250, clone 145-2C11, eBioscience, cat. 11-0031-63); PercP rat anti-mouse CD4 (1:250, clone RM4-5, BD Biosciences, cat. 553052); PE rat anti-mouse CD8a (1:250, clone 53-6.7, BD Biosciences, cat. 553033); Alexa Fluor® 647 rat anti-mouse Foxp3 (1:100, clone R16-715, BD Biosciences, cat. 563486); PE rat anti-CD11b (1:250, clone M1/70, BD Biosciences cat. 553311); PE hamster anti-mouse CD152/CTLA-4 Clone (1:150, UC10-4F10-11, BD Bioscience, cat. 553720); PE/Cy7 anti-mouse CD39 (1:250, clone Duha59 BioLegend, cat. 143806). For each sample, a minimum of 1 million events were acquired using a BD FACSVerse cytometer driven by the FACSuite software (BD Biosciences, San Diego, EUA). The obtained data were analyzed using the software FlowJo version X (Tree Star, Inc.). Gating strategies for flow cytometry analysis are schematically represented in Supplementary Fig. 11.
Heart CD11b+ and CD11b− cells isolation
The mouse heart tissue was sliced in small pieces and digested using Liberase TL (Roche) for 1 h at 37 °C/5% CO2. The obtained cell suspension was filtered through a 40-µm cell strainer (Corning®). Isolated cells were stained with PE rat anti-CD11b (1:300; clone M1-70, BD Biosciences, cat. 553311) and then incubated with anti-PE magnetic beads (Miltenyi Biotec). The cell suspension was separated into CD11b+ and CD11b− samples using MACS® cell separation columns (Miltenyi Biotec) according to the manufacturer’s instructions.
Total genomic DNA extraction and parasitism analysis
Total genomic DNA was extracted from 10 mg of CCC patients or mouse heart tissue or from mouse heart CD11b+ and CD11b− cells using a specific kit (Wizard® SV Genomic DNA Purification System Promega, cat. A2361) according to the manufacturer’s instructions. Real-time PCR was performed to quantify the heart parasitism as previously described48.
Treatment with dexamethasone
WT and Pik3cg−/− mice were infected with 103 trypomastigote forms of T. cruzi Y strain and treated intraperitoneally at day 9 post infection with 2 mg Kg− and at days 12 and 15 with 1 mg Kg− of dexamethasone or vehicle.
Treatment with benznidazole
Pik3cg−/− mice were infected with 103 trypomastigote forms of T. cruzi Y strain and treated by gavage with 100 mg Kg− of Benznidazole (BNZ) or vehicle. Mice were treated once a day starting from the day 9 post infection for 10 days.
BM cells isolation and generation of chimeric mice
WT and Pik3cg−/− BM stem cells were obtained by flushing the femur. Briefly, the bone was surgically removed, and muscle tissue was scraped away from bone using a scissor and scalpel blade. Subsequently, the epiphysis was cut, and the stem cells were removed from the diaphysis by flushing with RPMI 1640 medium using a syringe with a 26-gauge needle. Cells were centrifuged at 500 × g 10 min at 4 °C, suspended in PBS, counted using trypan blue solution (Sigma-Aldrich®) and diluted at 2.5 × 107 ml− (5 × 106/200 µl) for intravenous injection. To generate the chimeras, 10–12-weeks-old WT and Pik3cg−/− mice were irradiated using a Cesium 137 source irradiator (Mark I model 25) at 9 Gy. On the day after irradiation, the mice were divided at the following groups: (1) WT mice repopulated with WT BM cells; (2) Pik3cg−/− mice repopulated with WT BM cells; and (3) Pik3cg−/− mice repopulated with Pik3cg−/− BM cells. After BM transplantation, the mice were treated for 15 days with the antibiotic Ciprofloxacin hydrochloride diluted in drinking water at 10 mg ml−. After 2 months (period required for BM engraftment), mice were infected with 500 trypomastigote forms of T. cruzi Y strain, and the survival rate was followed every day for 30 days.
Differentiation of BMDM and killing assay
BMDMs were obtained as previously described49 and used for the killing activity assay, release of T. cruzi assay or NO quantification after stimulation with IFNγ and T. cruzi. For the killing activity assay, BMDMs (1.4 × 106 ml−) were incubated overnight with different concentrations of IFNγ (0.1 and 1 ng ml−) and macrophages posteriorly were infected with T. cruzi at a MOI 3:1 ratio. After 4 h, the cells were washed to remove non-internalized parasites and incubated for an additional 48 h at 37 °C a 5% CO2. The macrophage killing activity was evaluated by counting of intracellular amastigote forms internalized per 150 cells. The counts were performed in a blinded manner. For the release of T. cruzi assay, 2 × 105 cells were incubated with 1 ng ml− of IFNγ and after 12 h were infected with T. cruzi at a MOI of 3:1. At days 4 and 5 post infection trypomastigote forms of the parasites released to the medium were counted50.
THP-1 cells differentiation and killing activity assay
Authenticated THP-1 cells (cat. TIB-202, ATCC®, Manassas, VA, USA) monocytes lineage was differentiated into macrophages using the method previously described by Daigneault et al51. Briefly, THP-1 cells were cultured with 200 nM of PMA (Sigma-Aldrich; Merck Millipore) for 3 h at 37 °C, 5% CO2. After incubation, PMA-containing medium was removed, cells were plated in 24-wells plate at 2 × 105/well and the cells were incubated for an additional 3 days. At the third day, THP-1 were treated with 1 µM of PI3Kγ inhibitor AS605240 and infected with T. cruzi at a MOI 3:1 ratio followed by an additional 48 h of incubation at 37 °C in a 5% CO2 incubator. After 48 h, the cells were fixed and stained with Panótico (Laborclin®). The macrophage killing activity was evaluated by counting (blinded) of intracellular amastigote forms internalized per 50 cells. These cells were not contaminated with mycoplasma.
Nitrite and nitrate quantification
The nitrite concentration in the culture supernatants of BMDM was determined using the conventional Griess reaction method52. For the nitrate quantification assay, heart samples removed near the papillary muscle were homogenized with a sonicator (Virsonic 100, Virtis, NY, USA) in 200 μl of cold 0.1 N acetic acid, centrifuged for 5 min (9300 g) and the supernatant used for measurement of nitrate and total protein by the Bradford method. Subsequently, 25 µl of supernatant was deproteinized with 50 µl of cold ethanol and maintained at −20 °C for 30 min. Then, the samples were centrifuged (9300 g, 5 min) and the nitrate content was determined using a chemiluminescent analyzer (Sievers 280 NO Analyzer, Boulder, CO, USA). The values are expressed in µM nitrate per μg of protein.
In vivo cytotoxicity assay of CD8+ cells
Eighteen dpi, WT and Pik3cg−/− mice intravenously received two populations of splenocytes from WT naive mice previously stained with two different concentrations of carboxyflourescein (CFSE—Sigma Aldrich®). The first population was stained with CFSE at 10 μM (CFSE high) and pulsed for 40 min with the T. cruzi peptide PA8, which is presented based on class I MHC as the target of CD8+ cells. The second population stained with CFSE at 1 μM (CFSE low) and not pulsed with any peptide was used as the control population. Recipient WT and Pik3cg−/− mice were sacrificed approximately 16 h after the cell transfer, and splenocytes were analyzed with a flow cytometer to determine the percentage of CFSE high and low populations.
CD4+CD25+ suppression assay
CD4+ T-cells were isolated by negative selection from lymph nodes of WT mice using CD4 MACS beads Multisort (Miltenyi Biotec), according to the manufacturer’s recommendations. Briefly, the non-CD4+ T-cells were labeled with a mix containing cocktail of biotin-conjugated antibodies and anti-biotin monoclonal antibodies conjugated to microbeads. The magnetically labeled cells were subsequently depleted by separation using AutoMacs Pro Separator Cell sorter (Miltenyi Biotec). Next, CD4+ cells obtained were stained with PE anti-mouse CD25 (1:200, clone PC61.5, eBioscience, cat. 12-0251-81) and the CD25+ PE-labeled cells were incubated with anti-PE microBeads and isolated by positive selection. Two distinct cell populations, CD4+CD25− (effectors T-cells) and CD4+CD25+ (Tregs) were obtained. Tregs were cultured with T effectors cells in a 96-well U-bottom plate (Costar®). The Teff cells were labeled with 1 μM Dye Efluor 670 (eBioscience) for 15 min at 37 °C, washed, and then cultured (1 × 105 cells per well) for 4 days with a graded number of Tregs (Teff:Treg: 1:1, 1:2, 1:4, and 1:8) in the presence of soluble Purified hamster anti-mouse CD3e (3 μg/ml, Clone 145-2C11, BD Bioscience, cat. 553057) and Purified hamster anti-mouse CD28 (1.5 μg/mL, Clone 37.51, BD Bioscience, cat. 553294). Proliferation of Teff cells was determined by dye dilution in FACS analysis. The results are expressed as the percentage of suppression under each Treg:Teff ratio using the following formula: [proliferation of Teff only–(proliferation of Teff + Treg)/proliferation of Teff only] × 100.
Patient samples and tissue collection
Experiments on human samples were performed in accordance with the ethical standards established in the Declaration of Helsinki. The protocol was approved by the Institutional Review Board of the School of Medicine of São Paulo (CAPPesq-protocol number 0265-10) and the Brazilian National Ethics in Research Commission (CONEP protocol number 009/2011). Written informed consent was obtained from the patients. Tissue specimens from the left ventricle free wall were obtained from individuals with end-stage heart failure at the moment of heart transplantation (DCM patients, age 41.1 ± 15.63 years; mean ± SD). All patients with CCC (age 46.1 ± 9.33 years; mean ± SD) were considered serologically positive for antibodies against T. cruzi based on the results of at least two of three independent tests. They underwent standard electrocardiography and echocardiography. They presented with typical electrocardiography findings and had severe ventricular dysfunction, with a left ventricular ejection fraction of <0.4. Similarly, human samples were obtained from patients with idiopathic DCM characterized by severe ventricular dysfunction, an absence of ischemic disease, and negative results of serologic tests for T. cruzi infection. Finally, control biopsy specimens were obtained from healthy hearts of organ donors (mean age 23 ± 4.69 years) for which there was no suitable recipient. Human experiments were blinded with respect to the samples group.
Whole-genome expression was performed with the SurePrint G3 Human Gene Expression 8 × 60K arrays (Agilent Technologies, Les Ulis, France), according to the manufacturer’s recommendations. Gene expression data were deposited in the GEO database (GSE84796 and GSE111544). Microarray analyses and signal normalization were performed with GeneSpring software (11.5.1, Agilent). For each sample, the P-value was obtained using the Student’s t-test and adjusted for the false discovery rate with the Benjamini–Hochberg method. Genes were considered differentially expressed if adjusted P-values were <0.05 and showed an absolute fold change >2.0.
Results are expressed as the mean ± s.e.m. for in vitro and in vivo experiments. The normal distribution of data was analyzed by D’Agostino and Pearson test. The data set obtained by experiments with mice or primary cells assumed a normal distribution. Differences were considered to be statistically significant with P < 0.05 by unpaired Student’s t-test or ANOVA followed by Bonferroni post test. Survival curves were evaluated using the log-rank/Mantel–Cox test. For analysis of the correlation, Pearson’s test was carried out. All statistical analyses were performed using GraphPad Prism Software 5 except for the analysis of correlation, for which SPSS was used. No statistical methods were used to predetermine the sample size. Variation within each data set obtained by experiments with mice or primary cells was assumed to be similar between genotypes since all strains were generated and maintained on the same pure inbred background (C57BL/6).
The data supporting the findings of this study are available within the article and its Supplementary Information files or from the corresponding authors on reasonable request. RNA expression data are available at the Gene Expression Omnibus repository (GSE84796); (GSE111544); and (GSE41089).
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The authors gratefully acknowledge the technical assistance of Cristiane Maria Milanezi, Wander Ribeiro, Ieda R. Schivo, Giuliana Bertozi, and Sérgio Rosa. We also thank Júlio Anselmo Siqueira for supervising the animal facility as well as providing all animals used in this study. The research leading to these results received funding from the São Paulo Research Foundation (FAPESP) under grant agreements no. 2012/14524-9 (Thematic Project to J.S.S.), 2013/08216-2 (Center for Research in Inflammatory Disease), from the University of São Paulo NAP-DIN under grant agreement no. 11.1.21625.01.0; and a CAPES Visiting Professor Grant no. 88881.068044/20 14-01. M.C.S. was supported by doctoral fellowship from the São Paulo Research Foundation Grant 2011/09488-0. C.C. was supported by the Institut National de la Santé et de la Recherche Médicale (INSERM), Aix-Marseille University (Direction des Relations Internationales), the USP-COFECUB program, the ARCUS II PACA Brésil program, and from the Laboratoire d’Excellence (LabEx) ParaFrap ANR-11-LABX-0024. E.C.N. and C.C. were recipient for an international program (Br-Fr-Chagas) funded by the French (ANR) and the Brazilian (FAPESP) science funding agencies.
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