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Transcriptome analysis of the effect of C-C chemokine receptor 5 deficiency on cell response to Toxoplasma gondii in brain cells

BMC Genomics volume 20, Article number: 705 (2019) Cite this article

Abstract

Background

Infection with Toxoplasma gondii is thought to damage the brain and be a risk factor for neurological and psychotic disorders. The immune response-participating chemokine system has recently been considered vital for brain cell signaling and neural functioning. Here, we investigated the effect of the deficiency of C-C chemokine receptor 5 (CCR5), which is previously reported to be associated with T. gondii infection, on gene expression in the brain during T. gondii infection and the relationship between CCR5 and the inflammatory response against T. gondii infection in the brain.

Results

We performed a genome-wide comprehensive analysis of brain cells from wild-type and CCR5-deficient mice. Mouse primary brain cells infected with T. gondii were subjected to RNA sequencing. The expression levels of some genes, especially in astrocytes and microglia, were altered by CCR5-deficiency during T. gondii infection, and the gene ontology and Kyoto Encyclopedia of Genes and Genomes analysis revealed an enhanced immune response in the brain cells. The expression levels of genes which were highly differentially expressed in vitro were also investigated in the mouse brains during the T. gondii infections. Among the genes tested, only Saa3 (serum amyloid A3) showed partly CCR5-dependent upregulation during the acute infection phase. However, analysis of the subacute phase showed that in addition to Saa3, Hmox1 may also contribute to the protection and/or pathology partly via the CCR5 pathway.

Conclusions

Our results indicate that CCR5 is involved in T. gondii infection in the brain where it contributes to inflammatory responses and parasite elimination. We suggest that the inflammatory response by glial cells through CCR5 might be associated with neurological injury during T. gondii infection to some extent.

Background

Toxoplasma gondii is a protozoan apicomplexan parasite that causes the parasitic disease, toxoplasmosis. It can infect all mammals and birds, commonly through contaminated food [1]. The oocysts in feces from the definitive feline host can also be a source of infection in intermediate hosts such as rodents, birds, livestock, and humans. In these hosts, oocysts transform into tachyzoites shortly after ingestion of contaminated soil, water or plant material. Following exposure to the parasite, infection is divided into acute and chronic stages. The acute stage is characterized by replication of the fast replicating forms of the parasite, the tachyzoites. In contrast, bradyzoites in tissue cysts are responsible for establishing chronic latent infections [1].

Contamination of meat with T. gondii bradyzoites represents a major source of human infections [2], and a third of the world’s population is reportedly chronically infected with this parasite [1]. Although the prevalence of latent infections can reach 70% in human populations [3], there is currently no treatment that targets bradyzoite-containing tissue cysts. Toxoplasmosis causes severe clinical diseases in immunocompromised individuals and congenital disorders in infants [4]. In immunocompetent humans, toxoplasmosis is generally asymptomatic, but in patients with acquired immune deficiency syndrome (AIDS), their immunocompromised state reactivates the parasites, leading to the development of toxoplasmosis [5]. Uncontrolled parasite replication can cause life-threatening brain damage characterized by brain abscesses and necrotic areas, and toxoplasmic encephalitis is one of the primary causes of death in HIV-infected people [6]. Primary infections with T. gondii in pregnant women can also cause hydrocephalus or developmental disorders in the developing fetus [1].

T. gondii is capable of infecting most nucleated cells in vitro [7]. However, acute infections stimulate immune responses in the host, and these responses suppress the proliferation of the parasites [8]. The interferon-gamma (IFN-γ)-mediated immune response is central to this parasite-suppressive response. Many pathogens have developed strategies to modulate host nuclear factor-kappa B (NF-κB) activation and the onwards recruitment and activation of immune cells, which results in enhanced survival of the pathogen. Evidence currently exists to support both inhibition and activation of the NF-κB pathway in the host cells by T. gondii [9, 10]. The resultant immune attack and stressed condition inactivate T. gondii in most parts of the body. However, the parasite can persist in the brain as encysted bradyzoites [5, 8].

The human brain cell population consists mainly of three types: astrocytes, microglia, and neurons. Astrocytes, which has the highest population in the brain, participate in many brain activities such as brain development [11] and neurotransmission [12]. Microglia are crucial for brain injury and disease [13, 14], and neurons are vital in brain function processes such as neurotransmission and neuroendocrine activities [12]. In the brain, the chemokine system participates in neuroinflammatory processes and the development and functioning of the central nervous system (CNS), which includes neuron-glia communication and neuroendocrine activity [15]. These brain cells can also become infected with T. gondii tachyzoites [16]. However, a previous in vivo study showed that T. gondii is primarily found in neurons, suggesting that neurons are the primary target cells for this parasite [17]. Controversy exists concerning the effect of T. gondii on astrocytes, which may serve as parasite proliferation recipients or protective immune response activators within the CNS [18]. Besides their role in triggering anti-parasite immunity in T. gondii infections, microglia may act as “Trojan horses” [19].

Previously, our group reported on the upregulation of immune response-associated genes and downregulation of neurological function-related genes in whole-brain gene expression profiling during T. gondii infection [20]. The upregulated genes included chemokines and chemokine receptors; specifically, C-C chemokine ligand 5 (Ccl5) and Ccr5. C-C chemokine receptor 5 (CCR5) has been mainly studied in the context of HIV infection [21]. This chemokine receptor is expressed in memory and effector T-lymphocytes, natural killer cells, monocytes, macrophages and immature dendritic cells. In these cell types, CCR5 regulates chemotaxis and cell activation, including during T. gondii infection [21]. In some previous studies, CCR5-deficient (KO) mice showed increased susceptibility to systemic T. gondii infections and an increased number of brain cysts, suggesting that CCR5 is required for innate immunity against T. gondii and parasite elimination [22,23,24]. CCR5 is also expressed in brain cells such as neurons, astrocytes, and microglia. Previous studies on non-infective CNS injury have suggested that CCR5 plays neuroprotective functions [25, 26]. CCR5 is also implicated in the neural function of nociception [27]. A previous clinical study also showed that people with CCR5 chemokine receptor gene polymorphisms have a greater risk of developing ocular toxoplasmosis maybe due to a strong and persistent inflammatory response in ocular tissue. However, a detailed association between the mechanism underlying the inflammatory response during T. gondii infection and the role of CCR5 in the brain remains unclear.

Here, we aimed to examine the effect of CCR5-deficiency on gene expression in the brain during T. gondii infection and to know the relationship between CCR5 and the inflammatory response against T. gondii infection in the brain. We profiled the gene expression patterns of primary brain cells exposed to T. gondii tachyzoites using RNA sequencing (RNA-seq). In vivo assays were then used to quantify the expression levels of the genes that appeared to be involved in the control of parasite proliferation and pathology in the mouse brain. We suggest that the inflammatory response through CCR5 might be associated with neurological injury during T. gondii infection to some extent.

Results

Gene expression in astrocytes during T. gondii infection was affected by CCR5-deficiency

Primary astrocytes from wild-type (WT) and CCR5KO mice were infected with T. gondii tachyzoites and subjected to RNA-seq followed by differential expression analysis. The analysis identified 115 genes that were upregulated by T. gondii infection but were impaired by CCR5-deficiency (Additional file 1: Table S1). The functions of these differentially expressed genes (DEGs) were assessed by gene ontology (GO) term enrichment analysis (Table 1, Additional file 2: Table S2). Among the genes in which upregulation during infection was impaired by CCR5-deficiency, overrepresented GO terms were associated with immune response and response to stress categories. Kyoto Encyclopedia of Genes and Genomes (KEGG) pathway enrichment analysis showed that immune-related pathways such as the TNF signaling pathway, NOD-like signaling pathway, and antigen processing and presentation pathways were activated via CCR5 during the T. gondii infections (Additional file 3: Table S3; Additional file 4: Figure S1).

Table 1 Top 5 GO terms overrepresented in DEGs in which upregulation during T. gondii infection was affected by CCR5-deficiency. To explore the functions of DEGs in which upregulation during infection was affected by CCR5-deficiency, GO term enrichment analysis was performed
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To investigate the functions affected by CCR5-deficiency in astrocytes in more detail, DEGs in which upregulation during infection was impaired by CCR5-deficiency were ranked according to the fold-changes, calculated by DESeq2, occurring between T. gondii-infected cells from WT and CCR5KO mice, and the expression profiles of the top 20 genes were compared (Fig. 1a). The top 20 upregulated genes included IFN-γ inducible genes (i.e., C3, Fas, Gbp4, Gbp5, Gbp6). NF-κB target genes (i.e., C3, Chi3l1, Fas, Gadd45β, Hmox1, Ptx3, Saa3, Tlr2) were also abundant in DEGs in which upregulation during infection was impaired by CCR5-deficiency.

Fig. 1
figure 1

Expression of the top 20 DEGs in which upregulation during T. gondii infection was impaired by CCR5-deficiency. DEGs were ranked according to the fold-changes between the infected wild-type (WT) vs. infected CCR5-deficient (KO) mice. a, astrocytes; b, microglia; c, neurons. Each bar represents the fold-change between uninfected vs. infected mice. The values under the gene symbols are the ratio of the fold-change between uninfected KO vs. infected KO to that between uninfected WT vs. infected WT. The area of low fold-change is enlarged in panel A and B

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Gene expression in microglia during T. gondii infection was affected by CCR5-deficiency

Primary microglia from WT and CCR5KO mice were infected with tachyzoites and subjected to RNA-seq followed by differential expression analysis. The analysis identified 93 genes that were upregulated by T. gondii infection but were impaired by CCR5-deficiency (Additional file 1: Table S1). The functions of these DEGs were reviewed by GO term enrichment analysis (Table 1, Additional file 2: Table S2). Among the genes in which upregulation during infection was impaired by CCR5-deficiency, overrepresented GO terms were associated with inflammatory response and cytokine production. In KEGG pathway enrichment analysis of these genes, immune-related pathways such as IL-17, TNF, and NF-κB signaling pathways were overrepresented (Additional file 3: Table S3, Additional file 5: Figure S2).

To better understand the functions affected by CCR5-deficiency in microglia, DEGs of upregulated genes during infection which were disrupted by CCR5-deficiency were ranked in the same way as described above, and the expression levels of the top 20 genes were compared (Fig. 1b). The top 20 upregulated DEGs included many NF-κB target genes (i.e., Adora2a, Csf2, Csf3, Cxcl1 Edn1, Il6, Penk, Ptgs2, Tnfsf15). In addition, CCR5-deficiency during infection affected the upregulation of cytokine genes such as Csf2, Csf3, Cxcl1, Edn1, and Il6 and other genes associated with immune response (i.e., Gimap6, Mcoln2) and migration (i.e., Cyfip2).

Gene expression in neurons during T. gondii infection was affected by CCR5-deficiency

Primary neurons from WT and CCR5KO mice were infected with tachyzoites and subjected to RNA-seq followed by differential expression analysis. The analysis identified only 10 genes in which upregulation was impaired by CCR5-deficiency and T. gondii infection (Additional file 1: Table S1). GO term enrichment and KEGG pathway analyses were not performed on neurons because the number of the DEGs was too small to estimate accurately.

To better understand the functions affected by CCR5-deficiency, the 10 DEGs of upregulated genes which were impaired by CCR5-deficiency were ranked in the same way as described above (Fig. 1c). These DEGs included genes related to the immune system or immune pathways (i.e., Cd209g, Cd209f, Cd300e, Fgl2, Nfkb2), signal transduction (i.e., Cd300e, Ms4a6d, Nfkb2, Sla), apoptosis (i.e., Cd300e, Nfkb2), T-cell activation (i.e., Cd300e, Sla), transcription factors (i.e., Nfkb2) and NF-κB targeted genes (i.e., Cd209g, Nfkb2).

In vivo analysis of brain tissue from infected mice

WT and CCR5KO mice were intraperitoneally injected with 1000 tachyzoites and monitored daily for 30 days. Both WT and CCR5KO mice died from 10 to 16 days post-infection (dpi), which is thought to be the acute phase of systemic infection with T. gondii. The survival rate at 30 dpi was significantly lower in the infected CCR5KO mice (3/9) than in the WT mice (8/10) (Fig. 2a). While the mouse body weight at 0 dpi did not differ significantly among four groups (i.e., uninfected WT, infected WT, uninfected CCR5KO, and infected CCR5KO), at 9 dpi, infection was found to have a significant effect on the body weight, but not the mouse genotype or the interaction between infection and mouse genotype (Fig. 2b). The number of parasites in the brain at 30 dpi was significantly lower in the CCR5KO mice than in the WT mice (p < 0.05) (Fig. 3a). Mice were also injected with a higher number of tachyzoites (5000 per mouse) and were sacrificed at 7 dpi. At the time point, there was no significant difference in the number of brain-located parasites between WT and CCR5KO (Fig. 3b).

Fig. 2
figure 2

Survival rate and body weight of the infected wild-type (WT) and CCR5-deficient (KO) mice. a Survival rate was monitored until 30 dpi (infected WT, n = 10 + 8; infected CCR5KO, n = 9 + 6). Survival rate was compared between groups using the log-rank test (*p < 0.05). b Body weight change was monitored until 9 dpi, the day before the infected group started to die (uninfected WT, n = 4; uninfected CCR5KO, n = 4; infected WT, n = 10; infected CCR5KO, n = 9). Each point represents the mean ± SD. The weight difference between 0 dpi and 9 dpi was compared using two-way ANOVA. Effect of infection on body weight was significant (*p < 0.0001) but not the mouse genotype or the interaction between infection and mouse genotype (p > 0.05)

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Fig. 3
figure 3

Parasite numbers in the brain in the in vivo experiment. Parasite numbers in the brain tissue from the T. gondii-infected wild-type (WT) and CCR5-deficient (KO) mice were determined by real-time quantitative PCR on the T. gondii B1 gene. a, 30 dpi; b, 7 dpi. Parasite numbers were compared using the student’s unpaired t-test between the WT and CCR5KO mice (*p > 0.05). Ct values higher than those for the uninfected samples were considered indicative of nonspecific amplification and were excluded from the plot. Each symbol represents the data point for one mouse, and the bars represent the mean value for all the group data points (uninfected WT, n = 3; uninfected CCR5KO, n = 3; infected WT, n = 5; infected CCR5KO, n = 7)

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To investigate the in vivo expression of genes in which upregulation during infection was significantly impaired by CCR5-deficiency in the in vitro transcriptomic analysis, brain tissues from T. gondii-infected WT and CCR5KO mice were subjected to reverse transcription quantitative polymerase chain reaction (RT-qPCR) (Fig. 4, Additional file 6: Figure S3). Based on the results of the present transcriptomic profiling, 10 genes which were highly induced by T. gondii infection and showed a large difference between the fold-changes of “uninfected WT vs. infected WT” and “uninfected KO vs. infected KO” were selected for astrocytes (Dusp15, Gbp4, Saa3, Spib, Ube2ql1) and microglia (Adora2a, Csf2, Csf3, Cxcl1, Ptgs2). Moreover, we tested seven genes (Chi3l1, Gbp5, Hmox1, Mcoln2, Nfkb2, Ptx3, Sla) considering their functions in immune and defense responses. Furthermore, we selected another seven genes (i.e., C1qa, Cd36, Gfap, Ifng, Irf4, Socs1, Tgfbi), which we identified in our previous study to be associated with brain pathology during subacute T. gondii infection [20]. The genes encoding CCR5 (Ccr5) and its ligands (Ccl3, Ccl4, Ccl5) were also tested.

Fig. 4
figure 4

Expression of DEGs identified from the transcriptomic analysis was examined in the brain in the in vivo experiment. The brains of the T. gondii-infected wild-type (WT) and CCR5-deficient (KO) mice were prepared to determine their mRNA levels. a, 30 dpi; b, 7 dpi. The mRNA levels were normalized by the β-actin (Actb) mRNA level in the corresponding sample. * and # represent significant differences between the two groups in Tukey’s test after two-way ANOVA (**** and #### p < 0.0001, *** and ### p < 0.001, ** and ## p < 0.01, * and # p < 0.05). Each symbol represents the data point for one mouse, and the bars represent the mean value for all the group data points (uninfected WT, n = 4; uninfected CCR5KO, n = 4; infected WT, n = 5; infected CCR5KO, n = 5)

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At 30 dpi, the expression of 5 genes (Ccl4, Cd36, Hmox1, Saa3, Tgfbi) showed a significant interaction between mouse genotype and T. gondii infection (p < 0.05), thus revealing the existence of a partly CCR5-dependent immune response in the T. gondii-infected brain (Fig. 4a). Among these five genes, the results for Hmox1 and Saa3 were consistent with the transcriptome analysis for astrocytes. In contrast, the gene expression pattern in the brain at 7 dpi was not in agreement with the transcriptome analysis results for each cell type, except for Saa3 in astrocytes (Fig. 4b).

Discussion

In this study, we profiled the gene expression patterns of primary brain cells exposed to T. gondii tachyzoites using RNA-seq. Genes in which upregulation during infection was impaired by CCR5-deficiency were subsequently examined in vivo to quantify their expression levels and to investigate their potential involvement in the control of parasite proliferation and pathology in the mouse brain.

For astrocytes, among the genes in which upregulation during infection was impaired by CCR5-deficiency, overrepresented GO terms and KEGG pathways were associated with immune response and response to stress categories. This suggested that CCR5 has a role in the immune response in astrocytes during T. gondii infection. The top 20 upregulated genes included IFN-γ inducible genes (i.e., C3, Fas, Gbp4, Gbp5, Gbp6). Guanylate binding protein (GBP) genes located on chromosome 3, including Gbp5, play a critical role in the destruction of the parasitophorous vacuole membrane (PVM), along with interferon-inducible immunity-related GTPases (IRGs) [5, 28]. Gbp5 is IFN-γ inducible in astrocytes and participates in activating the nucleotide-binding oligomerization domain-like receptor protein 3 (NLRP3) inflammasome, a multiprotein oligomer responsible for activating inflammatory processes [29, 30]. Gbp genes located on chromosome 5, such as Gbp4 and Gbp6, are also IFN-γ inducible, but their role in astrocytes and during T. gondii infection is not well studied. During viral infection, GBP4 negatively regulates virus-induced type I IFN and antiviral response by interacting with IFN regulatory factor (IRF) 7 [31]. CCR5 is probably associated with parasite elimination by these GBPs in astrocytes. It is still unclear whether these IFN-γ inducible genes were induced with or without IFNs. Among the IFNs, only IFN-β (encoded by Ifnb1) was detected in RNA-seq in astrocytes although the mean normalized counts were quite low (4.5 ± 2.0 in infected WT and 1.8 ± 3.0 in infected KO). IFN-β is known to induce some anti-T. gondii genes [32]. Another possibility is that the IFN-γ inducible genes were induced without IFNs. It is known that some IFN-γ inducible genes are induced by signal transducers and activators of transcription 1 (STAT1), and T. gondii can phosphorylate STAT1 without IFNs [33]. Our results suggest that the mechanisms used for killing intracellular parasites partially depend on CCR5 in astrocytes.

In addition, NF-κB target genes (i.e., C3, Chi3l1, Fas, Gadd45β, Hmox1, Ptx3, Saa3, Tlr2) were abundant in the DEGs in which upregulation during infection was impaired by CCR5-deficiency. The current results suggest that signal transduction via CCR5 leads to activation of NF-κB during T. gondii infection in astrocytes, although CCR5 involvement in NF-κB activation is complicated as follows. The HIV envelope gp120 protein reportedly activates NF-κB via CCR5, but CCL4, a natural ligand for CCR5, did not activate NF-κB [34]. Another ligand, CCL5, activates NF-κB and induces cell migration in human osteosarcoma [35].

For microglia, among the DEGs which were upregulated during infection and were impaired by CCR5-deficiency, overrepresented GO terms were associated with immune response and cytokine production, and KEGG pathway enrichment analysis showed immune-related pathways such as IL-17, TNF, and NF-κB signaling pathways. CCR5 may participate in some of the functions in microglia such as cell processes including the regulatory processes essential for tissue development, architectural refinement, neural environment maintenance, response to injury and subsequent remodeling and repair [36]. A previous study showed that CCR1, CCR5, and CXCR2 chemokine receptors were functionally expressed on microglia [37]. With activated microglia, CCR5 is suggested to be responsible for changing the secretion levels of IL-10, insulin-like growth factors, and nitric oxide (NO) when engaged by CCL5 [37]. Our GO term analysis results regarding DEGs in which upregulation during infection was impaired by CCR5-deficiency are similar to previous reports about microglia functions [36, 37], suggesting that CCR5 has an effect on immune responses in microglia during T. gondii infection.

The top 20 upregulated DEGs in microglia included many NF-κB target genes (i.e., Adora2a, Csf2, Csf3, Cxcl1 Edn1, Il6, Penk, Ptgs2, Tnfsf15). Among the NF-κB target genes, Csf2, Csf3, Cxcl1, Edn1, and Il6 are cytokines. Cxcl1, a pro-inflammatory cytokine, is a known M1 macrophage-producing chemokine [38]. In M1 cells, the Toxoplasma dense granule protein GRA15-dependent induction of Cxcl1 has been reported [39]. Microglia and macrophages are mesodermal in origin [40], and pro-inflammatory M1 microglia may be capable of expressing this chemokine. Granulocyte-macrophage colony-stimulating factor (encoded by Csf2) has numerous effects on microglia, ranging from induction of proliferation to changes in morphology, and also increases lipopolysaccharide-induced production of proinflammatory mediators via TLR4 [41, 42]. Granulocyte colony-stimulating factor (encoded by Csf3), which was also identified as a factor produced by Toll-like receptor (TLR) 4-activated microglia, might contribute to oligodendrocyte progenitor cell proliferation or differentiation [43]. Because T. gondii is recognized by host TLRs including TLR4 [44], CCR5 may be involved in a pathogen recognition mechanism in microglia via TLR4. Thus far, the downstream signaling pathway via CCR5 remains obscure, especially in brain cells. Our results suggest that CCR5 may be involved in NF-κB activation in microglia during T. gondii infections, leading to expression of pro-inflammatory cytokines and chemokines. Furthermore, a previous study showed that deletion of NF-κB signaling in microglia rescued motor neurons from microglial-mediated death in vitro and extended survival in mice with amyotrophic lateral sclerosis by impairing pro-inflammatory microglial activation [45]. It is possible that activating NF-κB in microglia leads to tissue injury in the T. gondii-infected brain and causes neurological dysfunctionality. Future studies on the signaling pathway downstream of CCR5 and its relationship with NF-κB will provide better insight into the detailed mechanism underlying the functional role of CCR5.

Upregulation of some immune-related genes in neurons was also impaired by CCR5-deficiency. Among the upregulated DEGs in neurons, Nfkb2 and Cd209g are NF-κB target genes. Nfkb2, which encodes the NF-κB p100 subunit, is required for the canonical activation pathway. A direct role for Nfkb2 in the immune response against T. gondii has been described in the Nfkb2−/− mouse model, in which severe Toxoplasma encephalitis develops [46]. Murine CD209g shares structural and sequence homology with human CD209, which belongs to the family of C-type lectins that participate in innate immune responses by binding and clearing pathogens. In neurons, however, the level of perturbation by CCR5-deficiency was quite low, and the number of genes upregulated in a partly CCR5-dependent manner was much smaller compared with the results in astrocytes and microglia. Although this result might be because of the different multiplicity of infection, there is another possibility that involvement of CCR5 in the immune response to T. gondii infection in neurons differs from that in astrocytes and microglia, and that the host defense mechanism in neurons is less dependent on CCR5 than in astrocytes and microglia during infection. NF-κB has diverse functions, depending on the cellular context. Constitutively activated NF-κB is detected mostly in neurons, whereas NF-κB in glia has a lower basal activity and is heavily inducible. NF-κB function in neurons is responsible for learning and memory rather than inflammatory processes [47]. This could have something to do with neurons as a primary target cell of chronic infection of T. gondii. The roles performed by the upregulated DEGs against T. gondii infection in neurons warrant further study.

In in vivo assays, our result showed no significant difference in the number of brain-located parasites at 7 dpi between the WT and CCR5KO mouse groups. This result at 7 dpi is consistent with a previous study [24]. On the other hand, at 30 dpi, the number of parasites in the brain was significantly lower in the CCR5KO mice than in the WT mice. Contrary to our result, a previous report revealed that cyst numbers in the brain were higher in CCR5KO mice (C57BL/6 × 129 background) than in WT mice [22]. In addition to the difference in the background of mice, the difference between the present and previous studies could be due to the different methodology: timing of brain collection (30 dpi vs. at 18 dpi); parasite strain used (PLK strain vs. ME-49 strain); parasite life stage (1000 tachyzoites vs. 20 cysts). The susceptible mice died during the acute phase of T. gondii infections, which may be why the CCR5KO-infected mice harbored fewer parasites than the WT mice. Moreover, the CCR5KO mice showed significantly lower survival rate after infection. This may be due to the impaired immune response outside the brain; thus, we did not focus on the different survival rates in this study. Furthermore, our results revealed no significant differences in the number of brain-located parasites at 7 dpi between WT and CCR5KO.

Our current transcriptome analysis for primary brain cells showed that some genes were considered to be at least partly involved in the CCR5-dependent cellular response, which simultaneously suggests the involvement of CCR5 in brain pathology during T. gondii infection. Saa3, which was induced during acute and chronic inflammatory responses, encodes one of the primary acute-phase reactants, serum amyloid A (SAA) proteins. SAA is reported to prime NLRP3-inflammasome-dependent responses in macrophages [48, 49] and synovial fibroblasts [50], but its effect on brain glia is unknown [51]. Saa3 is predominantly expressed in macrophages [52], and the mRNA is induced in many tissues and is expressed at various levels in several different cell types [53]. Macrophages are a principal cell type that express extrahepatic Saa3 [53]. In the present study, Saa3 was upregulated in the brain tissues of T. gondii-infected mice, which might be related to its expression level in astrocytes and/or infiltrated peripheral blood immune cells. At 7 dpi, Saa3 expression in the brain was probably upregulated in response to the immune response against systemic infection with T. gondii, and this response possibly continued until 30 dpi. From the acute to subacute phase, Saa3 may play a role in promoting inflammation, similar to that which occurs in cancer metastasis [54], which is likely to depend on CCR5.

Upregulation of Hmox1 during infection with T. gondii was also impaired by CCR5-deficiency at 30 dpi. The protein encoded by the Hmox1 gene participates in cellular defenses against oxidative stress [55]. In response to an immune stimulus, glial cells, specifically astrocytes and microglia, become activated in the process termed gliosis [56] and stimulate the acute-phase response characterized by the release of cytokines, proteases, prostaglandins, and NO via increased expression of iNOS, and by stimulating the arachidonic acid cascade with increased production of reactive oxygen species (ROS) [57]. Oxidative stress injury is consistently linked to bipolar disease and toxoplasmosis. A cross-sectional study has investigated the possible role of Toxoplasma-induced oxidative stress in the development of bipolar disorders [58]. Also, Hmox1 is reportedly associated with cellular protection against oxidative stress [59] and indoleamine 2,3-dioxygenase (IDO) induction [60]. These findings suggest that Hmox1 may help to protect host cells from oxidative stress via an anti-parasitic mechanism (e.g., NO production and ROS production) [61] and that the attenuation may be partly dependent on CCR5. Meanwhile, most of the tested genes showed a low consistency between in vitro and in vivo experiments. This could be due to the different length of post-infection time between experiments (24 h vs. ≥7 days). We set the time points because our preliminary data showed that it takes about 7 days for parasite tachyzoites to start the invasion into the brain after intraperitoneal injection, but it seems there are still some gaps between in vitro and in vivo. Further studies would be required to clarify these findings.

Conclusions

This study is the first transcriptomic report on the relationship between CCR5 and T. gondii infection in primary brain cells and brain tissue. During T. gondii infection, expression levels of many genes associated with the immune response were affected by CCR5-deficiency. Our transcriptome result from purified primary cell cultures has provided new insight into the onset of local infection in each brain cell type and the involvement of CCR5. Many other factors could also influence the effect of T. gondii infection in brain tissue, including infiltration of immune cells from peripheral blood and cell-cell communications. We did not perform perfusion to remove the components in the peripheral blood due to a technical limitation, which might have resulted in an underestimation of changes in the brain in this study.

Because of its biological and anatomical complexity, in this study, the brain tissue showed expression patterns different from those of the primary brain cells, and differential expression by CCR5-deficiency was hardly detectable during the acute infection phase (7 dpi). In a tissue-level experiment, the effect of CCR5-deficiency on a cellular level should be covered and compensated, which might have contributed to our difficulty in observing gene expression difference between WT and CCR5KO mice in vivo. Nevertheless, our overall results suggest the involvement of CCR5 in the mouse brain during the subacute infection phase (30 dpi). Notably, the expression patterns of Saa3 and Hmox1 were consistent with the transcriptome analysis and the in vivo study at 30 dpi. This is the first study documenting the participation of these two genes in the CCR5 signaling pathway. Our data, which provides essential information on the involvement of CCR5 in neurological alteration and host protection from T. gondii, will assist further studies in elucidating its precise function.

Methods

Animals

C57BL/6 J mice were obtained from Clea Japan (Tokyo, Japan) and used as WT mice in this study. CCR5KO mice (B6.129P2-Ccr5tmlKuz/J, Stock No. 005427) were purchased from the Jackson Laboratory (Bar Harbor, ME, USA). Differential gene expressions due to the different parental strains were minimized by backcrossing the stock of CCR5KO mice to C57BL/6 eleven times in total before being imported into our laboratory. For the initial preparations of brain cells, mice at 6–8 weeks old were used as parents. Mice of 9–10 weeks old were used for in vivo experiments. All animals were housed in cages (6 mice/cage, 225 mm × 340 mm × 155 mm) with wood chips under specific-pathogen-free conditions in the animal facility of the National Research Center for Protozoan Diseases at Obihiro University of Agriculture and Veterinary Medicine, Hokkaido, Japan.

Preparation of T. gondii tachyzoites

T. gondii tachyzoites (PLK strain, type II) were maintained by serial passage on Vero cell monolayers at 37 °C in humidified air with 5% CO2. Parasites were washed by centrifugation, host cell debris was removed, and the parasites were resuspended in cold phosphate-buffered saline. Clustered cells and debris were removed by repeatedly passing the suspension through a 27-gauge needle and filtration through a 5.0-μm pore-size filter (Millipore, Burlington, MA, USA).

Cultures of astrocytes, microglia and neurons

Astrocytes, microglia and neurons were obtained from the brain cortices of fetal mice (age, E17–18) according to a previously described procedure [62, 63], with some modifications. Further details of the cultures can be found in Additional file 7: Supplemental Methods.

In vitro infection and RNA extraction

Primary brain cells were infected with T. gondii tachyzoites suspended in the medium appropriate for each cell type. Multiplicities of infection were 0.2, 1.0, and 1.0 for neurons, astrocytes, and microglia, respectively. Infected and uninfected groups of cells were prepared in triplicate wells for each mouse genotype and each cell type. After 24 h of infection, total RNA was extracted from individual wells of the monolayer cell samples with TRI reagent (Sigma-Aldrich, St. Louis, MO, USA), according to the manufacturer’s protocol. RNA extracted from each well was individually subjected to RNA-seq.

RNA-seq analysis

Transcriptome sequencing was performed according to the protocol used in our previous study [20]. Briefly, 1 μg of total RNA was subjected to poly-A selection. Sequencing libraries were constructed using the TruSeq RNA Sample Prep Kit (Illumina, San Diego, CA, USA), while 36-bp single-end sequencing was performed using the Illumina Genome Analyzer IIx and TruSeq SBS Kit v5-GA (36-cycle) (Illumina), according to the manufacturer’s instructions. All treatments and subsequent analyses were performed on individual transcripts. The data of uninfected samples has also been used in our previously published article [64] because all the sample cells in this article were prepared in the same experimental batch in the previous article.

Identification of DEGs in which upregulation during T. gondii infection was impaired by CCR5-deficiency

Sequence tags were aligned using TopHat (version 1.3.3 doi:https://doi.org/10.1093/bioinformatics/btp120) and gene transfer format (gtf) data (Mus_musculus.GRCm38.69), as previously described [20]. Raw sequence reads were mapped to the mouse genome (mm10, http://hgdownload.cse.ucsc.edu/downloads.html#mouse) with a two mismatches allowance. Based on the mapping results, differential expression analysis was performed for pairwise comparisons of the expression data using the R packages DESeq2 [65] and edgeR [66, 67]. In this study, only genes which appeared differentially expressed in both DESeq2 and edgeR were considered as DEGs. DEGs in which upregulation during infection was impaired by CCR5-deficiency were defined as follows: (1) log2 fold-change > 1 and FDR < 0.05 between the infected and uninfected WT mice; (2) FDR < 0.05 between the infected WT and CCR5KO mice; (3) the fold-change was higher in “uninfected WT vs. infected WT” than in “uninfected KO vs. infected KO”. Minor expressed genes were excluded by using cut-off values of ≤100 mean normalized counts in the infected WT mice for upregulated genes. As we aimed to investigate the effect of CCR5 on the expression of genes during T. gondii infection, we focused on DEGs in which upregulation during T. gondii infection was impaired by CCR5-deficiency although some genes were up/downregulated just by CCR5-deficiency regardless of T. gondii infection (Additional file 8: Table S4). For comparison among four groups (i.e., uninfected WT, infected WT, uninfected CCR5KO, and infected CCR5KO), the raw-read counts for each gene were normalized by the iDEGES method implemented in the TCC package [68]. Mouse Genome Informatics (MGI) data were obtained from the Mouse Genome Informatics database [69]. The expression of Ccr5 in each cell type was shown in Additional file 9: Figure S4.

GO analysis of DEGs in which upregulation during T. gondii infection was impaired by CCR5-deficiency

The DEGs in which upregulation during T. gondii infection was impaired by CCR5-deficiency were functionally categorized by GO term enrichment analysis. Statistical overrepresentation of GO terms for selected genes was compared with the reference genes (all genes; 37,315 genes) using the goseq package in R software [70]. Genome-wide annotation for mouse was obtained using the org.Mm.eg.db package [71]. Functional annotation charts for the enriched GO terms were generated using the GO terms associated with biological processes. Only GO terms with FDRs < 0.05 and the number of DEGs ≥10 were considered to represent functional enrichment.

KEGG pathway enrichment analysis

The KEGG database is a bioinformatics tool which assembles large-scale molecular datasets, like gene lists, into biological pathway maps [72]. The host DEGs list was subjected to KEGG pathway enrichment analysis using the clusterProfiler package [73] in the statistical environment R to assess their overarching functions. After counts per million normalization, the expression level of each gene in the enriched pathway was normalized by Z-score normalization and then visualized. Normalized gene expression was visualized in a heatmap using the heatmap.2 function [74] in the gplots package in R. Genes were hierarchically clustered based on the 1-Pearson correlation distance and group average method.

In vivo infections and brain collections

WT and CCR5KO mice were anesthetized with isoflurane (4% for 1 min) and then intraperitoneally injected with 1000 tachyzoites suspended in 400 μL of Roswell Park Memorial Institute (RPMI)-1640 Medium (Sigma-Aldrich). Their survival was monitored until 30 dpi. Each strain of mice was randomly allocated to uninfected and infected groups. Mice in uninfected groups were injected with RPMI-1640 Medium only. Data from two independent experiments were combined (uninfected WT, n = 4 + 4; uninfected CCR5KO, n = 4 + 4; infected WT, n = 8 + 10; infected CCR5KO, n = 6 + 9). In the second experiment, the mice body weights were monitored daily (uninfected WT, n = 4; uninfected CCR5KO, n = 4; infected WT, n = 10; infected CCR5KO, n = 9). After the experimental period, surviving mice were euthanized by cervical dislocation and then dissected. A half brain from each surviving mouse was harvested at 30 dpi (uninfected WT, n = 4; uninfected CCR5KO, n = 4; infected WT, n = 5; infected CCR5KO, n = 5), homogenized with BioMasher I (Nippi, Tokyo, Japan) and then subjected to RNA extraction with 2.5 ml of TRI reagent following the manufacturer’s protocol for tissue sample preparation and RNA isolation. The complementary DNA (cDNA) was prepared from 400 ng of RNA per reaction using PrimeScript™ II 1st strand cDNA Synthesis Kit (Takara Bio Inc., Shiga, Japan), following the manufacturer’s instructions.

Additionally, WT and CCR5KO mice were infected by intraperitoneal injections with a higher dose of tachyzoites (5000 tachyzoites per mouse) attempting to make the difference between WT and CCR5KO clear. The brains from these mice were harvested at 7 dpi (acute phase) when T. gondii tachyzoites typically start to invade into the brain. A half brain from each mouse was subjected to RNA extraction and cDNA preparation, as described above. The number of mice per group was as follows: uninfected WT, n = 3; uninfected CCR5KO, n = 3; infected WT, n = 9; infected CCR5KO, n = 8.

Reverse transcription quantitative PCR (RT-qPCR) for brain tissue analysis

The relative mRNA levels were calculated as described previously [64]. Primer sequences used for RT-qPCR were listed in Additional file 10: Table S5. Further details of the analyses can be found in Additional file 7: Supplemental Methods.

DNA extraction, quantitative PCR and T. gondii detection

The parasite number was calculated as described previously [64]. Further details of the analyses can be found in Additional file 7: Supplemental Methods.

Statistical analysis

Survival rate was compared between the WT and CCR5KO groups using the log-rank test. Regarding body weight change, weight differences between 0 dpi and 9 dpi were analyzed using two-way analysis of variance (ANOVA). Parasite numbers in the brain tissue were compared between the WT and CCR5KO mice at each dpi using the student’s unpaired t-test. Ct values higher than those for the uninfected samples were considered indicative of nonspecific amplification and were excluded from the analysis. Fisher’s exact test was performed to compare the percentage of mice with detectable brain parasites. mRNA levels were normalized against the β-actin (Actb) mRNA level in the corresponding sample and were compared between the WT and CCR5KO groups using Tukey’s test after two-way ANOVA.

Availability of data and materials

All data generated or analyzed during this study are included in this published article and its supplementary information files. The datasets are also available from the corresponding author on reasonable request.

Abbreviations

AIDS:

Acquired immune deficiency syndrome

ANOVA:

Analysis of variance

CCL:

C-C chemokine ligand

CCR:

C-C chemokine receptor

cDNA:

Complementary DNA

CNS:

Central nervous system

CYFIP2:

Cytoplasmic FMR1 interacting protein 2

DEG:

Differentially expressed gene

Dpi:

Days post infection

FDR:

False discovery rate

GBP:

Guanylate binding proteins

GO:

Gene ontology

Gtf:

Gene transfer format

IDO:

Indoleamine 2,3-dioxygenase

IFN:

Interferon

IL:

Interleukin

iNOS:

Inducible nitric oxide synthase

IRF:

Interferon regulatory factor

IRG:

Inducible immunity related GTPase

KEGG:

Kyoto Encyclopedia of Genes and Genomes

KO:

Knock-out

MGI:

Mouse Genome Informatics

NF-κB:

Nuclear factor-kappa B

NLRP3:

Nucleotide-binding oligomerization domain-like receptor protein 3

NO:

Nitric oxide

PVM :

Parasitophorous vacuole membrane

RNA-seq:

RNA sequencing

ROS:

Reactive oxygen species

RPMI:

Roswell Park Memorial Institute

RT-qPCR:

Reverse transcription quantitative chain polymerase reaction

SAA:

Serum amyloid A

STAT1:

Signal transducers and activators of transcription 1

TLR:

Toll-like receptor

WT:

Wild-type

References

  1. Montoya J, Liesenfeld O. Toxoplasmosis. Lancet. 2004;363:1965–76.

    Article  CAS  PubMed  Google Scholar 

  2. Jones JL, Dubey JP. Foodborne toxoplasmosis. Clin Infect Dis. 2012;55:845–51.

    Article  PubMed  Google Scholar 

  3. Pappas G, Roussos N, Falagas ME. Toxoplasmosis snapshots: global status of Toxoplasma gondii seroprevalence and implications for pregnancy and congenital toxoplasmosis. Int J Parasitol. 2009;39:1385–94.

    Article  PubMed  Google Scholar 

  4. Jones J, Lopez A, Wilson M. Congenital toxoplasmosis. Am Fam Physician. 2003;67:2131–8.

    PubMed  Google Scholar 

  5. Yarovinsky F. Innate immunity to Toxoplasma gondii infection. Nat Rev Immunol. 2014;14:109–21.

    Article  CAS  PubMed  Google Scholar 

  6. Basavaraju A. Toxoplasmosis in HIV infection: an overview. Trop Parasitol. 2016;6:129–35.

    Article  PubMed  Google Scholar 

  7. Joiner KA, Dubremetz JF. Toxoplasma gondii: a protozoan for the nineties. Infect Immun. 1993;61:1169–72.

    CAS  PubMed Central  PubMed  Google Scholar 

  8. Aliberti J. Host persistence: exploitation of anti-inflammatory pathways by Toxoplasma gondii. Nat Rev Immunol. 2005;5:162–70.

    Article  CAS  PubMed  Google Scholar 

  9. Shapira S, Speirs K, Gerstein A, Caamano J, Hunter CA. Suppression of NF-κB Activation by Infection with Toxoplasma gondii. J Infect Dis. 2002;185 Supplement_1:S66–S72.

    Article  CAS  PubMed  Google Scholar 

  10. Rosowski EE, Lu D, Julien L, Rodda L, Gaiser RA, Jensen KDC, et al. Strain-specific activation of the NF-κB pathway by GRA15, a novel Toxoplasma gondii dense granule protein. J Exp Med. 2011;208:195–212.

    Article  CAS  PubMed  Google Scholar 

  11. Hatten ME, Liem RKH, Shelanski ML, Mason CA. Astroglia in CNS injury. Glia. 1991;4:233–43.

    Article  CAS  Google Scholar 

  12. Araque A, Carmignoto G, Haydon PG. Dynamic signaling between astrocytes and neurons. Annu Rev Physiol. 2001;63:795–813.

    Article  CAS  Google Scholar 

  13. Kettenmann H, Hanisch U-K, Noda M, Verkhratsky A. Physiology of microglia. Physiol Rev. 2011;91:461–553.

    Article  CAS  PubMed  Google Scholar 

  14. Kreutzberg GW. Microglia: a sensor for pathological events in the CNS. Trends Neurosci. 1996;19:312–8.

    Article  CAS  PubMed  Google Scholar 

  15. Ambrosini E, Aloisi F. Chemokines and glial cells: a complex network in the central nervous system. Neurochem Res. 2004;29:1017–38.

    Article  CAS  PubMed  Google Scholar 

  16. Lüder CGK, Giraldo-Velásquez M, Sendtner M, Gross U. Toxoplasma gondii in primary rat CNS cells: differential contribution of neurons, astrocytes, and microglial cells for the intracerebral development and stage differentiation. Exp Parasitol. 1999;93:23–32.

    Article  PubMed  Google Scholar 

  17. Cabral CM, Tuladhar S, Dietrich HK, Nguyen E, MacDonald WR, Trivedi T, et al. Neurons are the primary target cell for the brain-tropic intracellular parasite Toxoplasma gondii. PLoS Pathog. 2016;12:e1005447.

    Article  PubMed  Google Scholar 

  18. Contreras-Ochoa CO, Lagunas-Martínez A, Belkind-Gerson J, Correa D. Toxoplasma gondii invasion and replication in astrocyte primary cultures and astrocytoma cell lines: systematic review of the literature. Parasitol Res. 2012;110:2089–94.

    Article  PubMed  Google Scholar 

  19. Dellacasa-Lindberg I, Fuks JM, Arrighi RBG, Lambert H, Wallin RPA, Chambers BJ, et al. Migratory activation of primary cortical microglia upon infection with Toxoplasma gondii. Infect Immun. 2011;79:3046–52.

    Article  CAS  PubMed  Google Scholar 

  20. Tanaka S, Nishimura M, Ihara F, Yamagishi J, Suzuki Y, Nishikawa Y. Transcriptome analysis of mouse brain infected with Toxoplasma gondii. Infect Immun. 2013;81:3609–19.

    Article  CAS  PubMed  Google Scholar 

  21. Sorce S, Myburgh R, Krause K-H. The chemokine receptor CCR5 in the central nervous system. Prog Neurobiol. 2011;93:297–311.

    Article  CAS  Google Scholar 

  22. Aliberti J, Sousa CR e, Schito M, Hieny S, Wells T, Huffnagle GB, et al. CCR5 provides a signal for microbial induced production of IL-12 by CD8α+ dendritic cells. Nat Immunol. 2000;1:ni0700_83.

    Article  CAS  Google Scholar 

  23. Bonfá G, Benevides L, Souza M. Do C, Fonseca DM, Mineo TWP, Rossi MA, et al. CCR5 controls immune and metabolic functions during Toxoplasma gondii infection. PLoS One. 2014;9:e104736.

    Article  PubMed  Google Scholar 

  24. Khan IA, Thomas SY, Moretto MM, Lee FS, Islam SA, Combe C, et al. CCR5 is essential for NK cell trafficking and host survival following Toxoplasma gondii infection. PLoS Pathog. 2006;2:e49.

    Article  PubMed  Google Scholar 

  25. Gamo K, Kiryu-Seo S, Konishi H, Aoki S, Matsushima K, Wada K, et al. G-protein-coupled receptor screen reveals a role for chemokine receptor CCR5 in suppressing microglial neurotoxicity. J Neurosci. 2008;28:11980–8.

    Article  CAS  PubMed  Google Scholar 

  26. Sorce S, Bonnefont J, Julien S, Marq-Lin N, Rodriguez I, Dubois-Dauphin M, et al. Increased brain damage after ischaemic stroke in mice lacking the chemokine receptor CCR5. Br J Pharmacol. 2010;160:311–21.

    Article  CAS  PubMed  Google Scholar 

  27. Lee YK, Choi D-Y, Jung Y-Y, Yun YW, Lee BJ, Han SB, et al. Decreased pain responses of C–C chemokine receptor 5 knockout mice to chemical or inflammatory stimuli. Neuropharmacology. 2013;67 Supplement C:57–65.

    Article  CAS  Google Scholar 

  28. Yamamoto M, Okuyama M, Ma JS, Kimura T, Kamiyama N, Saiga H, et al. A cluster of interferon-γ-inducible p65 GTPases plays a critical role in host defense against Toxoplasma gondii. Immunity. 2012;37:302–13.

    Article  CAS  Google Scholar 

  29. Hidano S, Randall LM, Dawson L, Dietrich HK, Konradt C, Klover PJ, et al. STAT1 Signaling in Astrocytes Is Essential for Control of Infection in the Central Nervous System. mBio. 2016;7:e01881–16.

    Article  CAS  PubMed  Google Scholar 

  30. Shenoy AR, Wellington DA, Kumar P, Kassa H, Booth CJ, Cresswell P, et al. GBP5 promotes NLRP3 Inflammasome assembly and immunity in mammals. Science. 2012;336:481–5.

    Article  CAS  PubMed  Google Scholar 

  31. Hu Y, Wang J, Yang B, Zheng N, Qin M, Ji Y, et al. Guanylate binding protein 4 negatively regulates virus-induced type I IFN and antiviral response by targeting IFN regulatory factor 7. J Immunol. 2011;187:6456–62.

    Article  CAS  PubMed  Google Scholar 

  32. Mahmoud ME, Ui F, Salman D, Nishimura M, Nishikawa Y. Mechanisms of interferon-beta-induced inhibition of Toxoplasma gondii growth in murine macrophages and embryonic fibroblasts: role of immunity-related GTPase M1. Cell Microbiol. 17:1069–83.

    Article  CAS  Google Scholar 

  33. Schneider AG, Abdallah DSA, Butcher BA, Denkers EY. Toxoplasma gondii triggers phosphorylation and nuclear translocation of dendritic cell STAT1 while simultaneously blocking IFNγ-induced STAT1 transcriptional activity. PLoS One. 2013;8:e60215.

    Article  CAS  PubMed  Google Scholar 

  34. Fantuzzi L, Spadaro F, Purificato C, Cecchetti S, Podo F, Belardelli F, et al. Phosphatidylcholine-specific phospholipase C activation is required for CCR5-dependent, NF-kB–driven CCL2 secretion elicited in response to HIV-1 gp120 in human primary macrophages. Blood. 2008;111:3355–63.

    Article  CAS  PubMed  Google Scholar 

  35. Wang S-W, Wu H-H, Liu S-C, Wang P-C, Ou W-C, Chou W-Y, et al. CCL5 and CCR5 interaction promotes cell motility in human osteosarcoma. PLoS One. 2012;7:e35101.

    Article  CAS  PubMed  Google Scholar 

  36. Orihuela R, McPherson CA, Harry GJ. Microglial M1/M2 polarization and metabolic states. Br J Pharmacol. 2016;173:649–65.

    Article  CAS  Google Scholar 

  37. Škuljec J, Sun H, Pul R, Bénardais K, Ragancokova D, Moharregh-Khiabani D, et al. CCL5 induces a pro-inflammatory profile in microglia in vitro. Cell Immunol. 2011;270:164–71.

    Article  PubMed  Google Scholar 

  38. Sica A, Mantovani A. Macrophage plasticity and polarization: in vivo veritas. J Clin Invest. 2012;122:787–95.

    Article  CAS  PubMed  Google Scholar 

  39. Jensen KDC, Wang Y, Wojno EDT, Shastri AJ, Hu K, Cornel L, et al. Toxoplasma polymorphic effectors determine macrophage polarization and intestinal inflammation. Cell Host Microbe. 2011;9:472–83.

    Article  CAS  PubMed  Google Scholar 

  40. Ginhoux F, Prinz M. Origin of microglia: current concepts and past controversies. Cold Spring Harb Perspect Biol. 2015;7:a020537.

    Article  PubMed  Google Scholar 

  41. Parajuli B, Sonobe Y, Kawanokuchi J, Doi Y, Noda M, Takeuchi H, et al. GM-CSF increases LPS-induced production of proinflammatory mediators via upregulation of TLR4 and CD14 in murine microglia. J Neuroinflammation. 2012;9:268.

    Article  CAS  PubMed  Google Scholar 

  42. Liva SM, Kahn MA, Dopp JM, Vellis JD. Signal transduction pathways induced by GM-CSF in microglia: significance in the control of proliferation. Glia. 1999;26:344–52.

    Article  CAS  PubMed  Google Scholar 

  43. Goldstein EZ. TLR4-activated microglia have divergent effects on oligodendrocyte lineage cells: The Ohio State University; 2016. https://etd.ohiolink.edu/pg_10?0::NO:10:P10_ACCESSION_NUM:osu1468967532.

  44. Wujcicka W, Wilczyński J, Nowakowska D. SNPs in toll-like receptor (TLR) genes as new genetic alterations associated with congenital toxoplasmosis? Eur J Clin Microbiol Infect Dis Off Publ Eur Soc Clin Microbiol. 2012;32.

    Article  Google Scholar 

  45. Frakes AE, Ferraiuolo L, Haidet-Phillips AM, Schmelzer L, Braun L, Miranda CJ, et al. Microglia induce motor neuron death via the classical NF-κB pathway in amyotrophic lateral sclerosis. Neuron. 2014;81:1009–23.

    Article  CAS  PubMed  Google Scholar 

  46. Caamaño J, Tato C, Cai G, Villegas EN, Speirs K, Craig L, et al. Identification of a role for NF-κB2 in the regulation of apoptosis and in maintenance of T cell-mediated immunity to Toxoplasma gondii. J Immunol. 2000;165:5720–8.

    Article  PubMed  Google Scholar 

  47. Kaltschmidt B, Kaltschmidt C. NF-κB in the nervous system. Cold Spring Harb Perspect Biol. 2009;1. https://doi.org/10.1101/cshperspect.a001271.

    Article  PubMed  Google Scholar 

  48. Ather JL, Ckless K, Martin R, Foley KL, Suratt BT, Boyson JE, et al. Serum Amyloid A (SAA) Activates the NLRP3 Inflammasome and Promotes TH17 Allergic Asthma in Mice. J Immunol Baltim Md 1950. 2011;187:64–73.

  49. Niemi K, Teirilä L, Lappalainen J, Rajamäki K, Baumann MH, Öörni K, et al. Serum amyloid a activates the NLRP3 Inflammasome via P2X7 receptor and a Cathepsin B-sensitive pathway. J Immunol. 2011;186:6119–28.

    Article  CAS  PubMed  Google Scholar 

  50. Migita K, Koga T, Satomura K, Izumi M, Torigoshi T, Maeda Y, et al. Serum amyloid a triggers the mosodium urate -mediated mature interleukin-1β production from human synovial fibroblasts. Arthritis Res Ther. 2012;14:R119.

    Article  CAS  PubMed  Google Scholar 

  51. Savage CD, Lopez-Castejon G, Denes A, Brough D. NLRP3-Inflammasome activating DAMPs stimulate an inflammatory response in glia in the absence of priming which contributes to brain inflammation after injury. Front Immunol. 2012;3. https://doi.org/10.3389/fimmu.2012.00288.

  52. Eckhardt ER, Witta J, Zhong J, Arsenescu R, Arsenescu V, Wang Y, et al. Intestinal epithelial serum amyloid a modulates bacterial growth in vitro and pro-inflammatory responses in mouse experimental colitis. BMC Gastroenterol. 2010;10:133.

    Article  PubMed  Google Scholar 

  53. Meek RL, Eriksen N, Benditt EP. Murine serum amyloid A3 is a high density apolipoprotein and is secreted by macrophages. Proc Natl Acad Sci U S A. 1992;89:7949–52.

    Article  CAS  PubMed  Google Scholar 

  54. Hiratsuka S, Watanabe A, Sakurai Y, Akashi-Takamura S, Ishibashi S, Miyake K, et al. The S100A8-serum amyloid A3-TLR4 paracrine cascade establishes a pre-metastatic phase. Nat Cell Biol. 2008;10:1349–55.

    Article  CAS  Google Scholar 

  55. Jazwa A, Cuadrado A. Targeting heme oxygenase-1 for neuroprotection and neuroinflammation in neurodegenerative diseases. Curr Drug Targets. 2010;11:1517–31.

    Article  CAS  Google Scholar 

  56. Andersson P-B, Perry VH. Gordon† S. the acute inflammatory response to lipopolysaccharide in cns parenchyma differs from that in other body tissues. Neuroscience. 1992;48:169–86.

    Article  CAS  Google Scholar 

  57. Gottschall PE, Komaki G, Arimura A. Increased circulating interleukin-1 and interleukin-6 after intracerebroventricular injection of lipopolysaccharide. Neuroendocrinology. 1992;56:935–8.

    Article  CAS  PubMed  Google Scholar 

  58. Afifi MA, Jiman-Fatani AA, Al-Rabia MW, Al-Hussainy NH, El Saadany S, Mayah W. More than an association: latent toxoplasmosis might provoke a local oxidative stress that triggers the development of bipolar disorder. J Microsc Ultrastruct. 2017. https://doi.org/10.1016/j.jmau.2017.05.003.

  59. Cerrito MG, Scagliarini A, Froio A, Liloia A, Busnelli M, Giovannoni R, et al. Heme oxygenase-1 inhibition prevents intimal hyperplasia enhancing nitric oxide-dependent apoptosis of vascular smooth muscle cells. Biol Pharm Bull. 2011;34:1204–14.

    Article  CAS  PubMed  Google Scholar 

  60. Oh G-S, Pae H-O, Choi B-M, Chae S-C, Lee H-S, Ryu D-G, et al. 3-Hydroxyanthranilic acid, one of metabolites of tryptophan via indoleamine 2,3-dioxygenase pathway, suppresses inducible nitric oxide synthase expression by enhancing heme oxygenase-1 expression. Biochem Biophys Res Commun. 2004;320:1156–62.

    Article  CAS  Google Scholar 

  61. Shrestha SP, Tomita T, Weiss LM, Orlofsky A. Proliferation of Toxoplasma gondii in inflammatory macrophages in vivo is associated with diminished oxygen radical production in the host cell. Int J Parasitol. 2006;36:433–41.

    Article  CAS  PubMed  Google Scholar 

  62. Fischer HG, Nitzgen B, Germann T, Degitz K, Däubener W, Hadding U. Differentiation driven by granulocyte-macrophage colony-stimulating factor endows microglia with interferon-gamma-independent antigen presentation function. J Neuroimmunol. 1993;42:87–95.

    Article  CAS  Google Scholar 

  63. Hilgenberg LGW, Smith MA. Preparation of dissociated mouse cortical neuron cultures. J Vis Exp JoVE. 2007. https://doi.org/10.3791/562.

  64. Umeda K, Tanaka S, Ihara F, Yamagishi J, Suzuki Y, Nishikawa Y. Transcriptional profiling of toll-like receptor 2-deficient primary murine brain cells during Toxoplasma gondii infection. PLoS One. 2017;12:e0187703.

    Article  PubMed  Google Scholar 

  65. Love MI, Huber W, Anders S. Moderated estimation of fold change and dispersion for RNA-seq data with DESeq2. Genome Biol. 2014;15:550.

    Article  PubMed  Google Scholar 

  66. McCarthy DJ, Chen Y, Smyth GK. Differential expression analysis of multifactor RNA-Seq experiments with respect to biological variation. Nucleic Acids Res. 2012;40:4288–97.

    Article  CAS  PubMed  Google Scholar 

  67. Robinson MD, McCarthy DJ, Smyth GK. edgeR: a Bioconductor package for differential expression analysis of digital gene expression data. Bioinformatics. 2010;26:139–40.

    Article  CAS  PubMed  Google Scholar 

  68. Tang M, Sun J, Shimizu K, Kadota K. Evaluation of methods for differential expression analysis on multi-group RNA-seq count data. BMC Bioinformatics. 2015;16:360.

    Article  Google Scholar 

  69. Eppig JT, Blake JA, Bult CJ, Kadin JA, Richardson JE. The mouse genome database (MGD): comprehensive resource for genetics and genomics of the laboratory mouse. Nucleic Acids Res. 2012;40:D881–6.

    Article  CAS  Google Scholar 

  70. Young MD, Wakefield MJ, Smyth GK, Oshlack A. Gene ontology analysis for RNA-seq: accounting for selection bias. Genome Biol. 2010;11:R14.

    Article  PubMed  Google Scholar 

  71. Carlson M, Falcon S, Pages H, Li N. org.Mm. eg. db: Genome wide annotation for Mouse. 2015.

  72. Kanehisa M, Sato Y, Kawashima M, Furumichi M, Tanabe M. KEGG as a reference resource for gene and protein annotation. Nucleic Acids Res. 2016;44:D457–62.

    Article  CAS  PubMed  Google Scholar 

  73. Yu G, Wang L-G, Han Y, He Q-Y. clusterProfiler: an R package for comparing biological themes among gene clusters. OMICS J Integr Biol. 2012;16:284–7.

    Article  CAS  Google Scholar 

  74. Warnes MGR, Bolker B, Bonebakker L, Gentleman R. Package ‘gplots.’ Var R Program Tools Plotting Data 2016.

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Acknowledgments

We thank the members of the Research Unit for Host Defense (National Research Center for Protozoan Diseases, Obihiro University of Agriculture and Veterinary Medicine) for their technical support with the mouse experiments, and the Center for Omics and Bioinformatics (Graduate School of Frontier Sciences, University of Tokyo) for the RNA sequencing and its related analysis. We thank Sandra Cheesman, Ph.D., from Edanz Group (www.edanzediting.com/ac) and Rochelle Haidee D. Ybañez (National Research Center for Protozoan Diseases, Obihiro University of Agriculture and Veterinary Medicine) for editing a draft of this manuscript.

Funding

This research was supported by the Japan Society for the Promotion of Science (JSPS) through the Funding Program for Next Generation World-Leading Researchers (NEXT Program), initiated by the Council for Science and Technology Policy (2011/LS003 [YN]), Grant-in-Aid for Exploratory Research JP15K15118 [YN] and Challenging Research (Exploratory) JP17K19538 [YN]), Grant-in-Aid for Young Scientists (B) JP17K17570 [KU] and a Research Program on Emerging and Re-emerging Infectious Diseases (17fk0108120h0001 [YN]) from Agency for Medical Research and Development (AMED). These funding bodies played no role in the design of the study and collection, analysis, and interpretation of data and in writing the manuscript.

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Author notes

  1. Kaoru Kobayashi and Kousuke Umeda contributed equally to this work.

Authors and Affiliations

  1. National Research Center for Protozoan Diseases, Obihiro University of Agriculture and Veterinary Medicine, Obihiro, Hokkaido, Japan

    Kaoru Kobayashi, Kousuke Umeda, Fumiaki Ihara & Yoshifumi Nishikawa

  2. Division of Animal Science, Department of Agricultural and Life Sciences, Faculty of Agriculture, Shinshu University, Minamiminowa, Nagano, Japan

    Sachi Tanaka

  3. Research Center for Zoonosis Control, Hokkaido University, Sapporo, Hokkaido, Japan

    Junya Yamagishi

  4. Graduate School of Frontier Science, The University of Tokyo, Kashiwa, Chiba, Japan

    Yutaka Suzuki

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  7. Yoshifumi Nishikawa
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Contributions

KK, KU. and YN conceived and designed the experiments and analyzed the data. KK, KU, FI, ST, JY, YS and YN performed the experiments and contributed the reagents. KK, KU and YN wrote the manuscript. All authors have read and approved the final manuscript.

Corresponding author

Correspondence to Yoshifumi Nishikawa.

Ethics declarations

Ethics approval and consent to participate

Our study was performed in strict accordance with the recommendations of the Guide for the Care and Use of Laboratory Animals of the Ministry of Education, Culture, Sports, Science and Technology, Japan. The protocol was approved by the Committee on the Ethics of Animal Experiments at Obihiro University of Agriculture and Veterinary Medicine (permit number 29–59). All surgeries were performed under isoflurane anesthesia with every effort made to minimize animal suffering. The study also adhered to the ARRIVE guidelines for reporting in vivo animal experiments (Additional file 11).

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Not applicable.

Competing interests

The authors declare that they have no competing interests.

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Supplementary information

Additional file 1: Table S1.

Detailed expression data for DEGs in which upregulation during T. gondii infection was impaired by CCR5-deficiency. (XLSX 67 kb)

Additional file 2: Table S2.

Detailed data for top 10 GO terms overrepresented in the DEGs in which upregulation during T. gondii infection was impaired by CCR5-deficiency in astrocytes and microglia. (XLSX 12 kb)

Additional file 3: Table S3.

Top10 KEGG pathways enriched in the DEGs in which upregulation during T. gondii infection was impaired by CCR5-deficiency in astrocytes and microglia. (XLSX 11 kb)

Additional file 4: Figure S1.

Expression patterns of genes in the TNF signaling pathway in astrocytes. The enlarged area shows the genes thought to be affected by CCR5-deficiency. (TIF 826 kb)

Additional file 5: Figure S2.

Expression patterns of genes in the IL-17 signaling pathway in microglia. The enlarged area shows the genes thought to be affected by CCR5-deficiency. (TIF 874 kb)

Additional file 6: Figure S3.

Gene expression in the brain of T. gondii-infected mice. Genes with no significant interactions between mouse genotype and infection in a two-way ANOVA are shown. Each symbol represents the data point for one mouse, and the bars represent the mean value for all the group data points. A, 30 dpi (uninfected wild-type mice (WT), n = 4; uninfected CCR5-deficient mice (CCR5KO), n = 4; infected WT, n = 5; infected CCR5KO, n = 5); B, 7 dpi (uninfected WT, n = 3; uninfected CCR5KO, n = 3, infected WT, n = 5; infected CCR5KO, n = 7). (TIF 970 kb)

Additional file 7:

Supplemental Methods. (DOCX 26 kb)

Additional file 8: Table S4.

Genes up/downregulated just by CCR5-deficiency regardless of T. gondii infection. DEGs were identified by comparing between the uninfected wild-type and uninfected CCR5-deficient mice, with a threshold of 2-fold change and < 0.05 false discovery rate. (XLSX 114 kb)

Additional file 9: Figure S4.

Expression of Ccr5 in astrocytes, microglia, and neurons in the transcriptomic analysis. A, astrocytes; B, microglia; C, neurons. Each bar represents the mean ± SD (n = 3), which were calculated after normalizing the raw-read counts using the iDEGES method. (TIF 1167 kb)

Additional file 10: Table S5.

Primer sequences used in RT-qPCR. (XLSX 11 kb)

Additional file 11:

The ARRIVE Guidelines Checklist. (PDF 1093 kb)

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Kobayashi, K., Umeda, K., Ihara, F. et al. Transcriptome analysis of the effect of C-C chemokine receptor 5 deficiency on cell response to Toxoplasma gondii in brain cells. BMC Genomics 20, 705 (2019). https://doi.org/10.1186/s12864-019-6076-4

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Keywords

BMC Genomics

ISSN: 1471-2164

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