Abstract
Toxoplasma (T.) gondii is an obligate intracellular parasite with a worldwide distribution. Congenital infection can lead to severe pathological alterations in the brain. To examine the effects of toxoplasmosis in the fetal brain, pregnant guinea pigs are infected with T. gondii oocysts on gestation day 23 and dissected 10, 17 and 25 days afterwards. We show the neocortex to represent a target region of T. gondii and the parasite to infect neural progenitor cells (NPCs), neurons and astrocytes in the fetal brain. Importantly, we observe a significant reduction in neuron number at end-neurogenesis and find a marked reduction in NPC count, indicating that impaired neurogenesis underlies the neuronal decrease in infected fetuses. Moreover, we observe focal microglioses to be associated with T. gondii in the fetal brain. Our findings expand the understanding of the pathophysiology of congenital toxoplasmosis, especially contributing to the development of cortical malformations.
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Introduction
The obligate intracellular parasite Toxoplasma (T.) gondii causes the zoonosis toxoplasmosis1,2,3. In humans, the worldwide seroprevalence of T. gondii is approximately 33%4,5. Around 1.9% of women of childbearing age become infected for the first time during pregnancy5. All warm-blooded animals can serve as intermediate hosts and members of the cat family (Felidae) are the definitive hosts of T. gondii. The life cycle of T. gondii consists of different developmental stages6,7. This parasite reproduces sexually in the intestinal epithelium of the definitive host, which results in the excretion of oocysts in the feces8 In the external environment, during a process called sporulation, infective sporozoites develop within the oocysts. Oral infection of the intermediate host leads to rapid asexual proliferation of the acute (tachyzoite) stage7,9. After infection, T. gondii tachyzoites disseminates through the infected host via blood, lymph or other body fluids, able to reach all host tissues. About 10–14 days after infection, the immune response of the host against T. gondii has developed and causes chronic infection, which is characterized by intracellular tissue cysts, harboring bradyzoites, which may remain in the host for life, especially in the brain, retina, skeletal, and cardiac muscle cells7,10,11,12,13. Primary routes of infection of the intermediate host are insufficiently heated or raw meat containing tissue cysts and ingestion of water or food contaminated with sporulated oocysts14,15,16.
Importantly, the parasite is able to cross the placental barrier during maternal parasitemia and subsequently infect the embryo/fetus after primary infection of the mother1,3,17. In healthy and immunocompetent adults, the infection is usually asymptomatic. However, congenital infection may lead to severe symptoms in the offspring, especially in the brain6,18. The clinical picture of human congenital toxoplasmosis depends on the time of infection during pregnancy. An infection in early gestation, especially in the first trimester may lead to abortion. Infection in mid gestation is often characterized by microcephaly, intellectual disability, and retinochorioiditis, while congenital infection in the third trimester of pregnancy may result in cerebral calcifications and hepatosplenomegaly19,20.
Data from in vitro experiments and adult mouse models have shown that T. gondii is able to infect neurons and astrocytes, leading to impairments in the number, morphology and function of the infected cells21,22,23,24,25,26,27,28. In eutherian mammals, neurogenesis occurs predominantly before birth and therefore neural stem and progenitor cells (NPCs) are exclusively present in high abundance in the prenatal cortex. Based on location of their nucleus at mitosis, NPCs can be divided into two major classes: apical progenitors (APs) and basal progenitors (BPs)29,30,31,32,33,34. APs are the primary NPCs, whose cell body resides in the ventricular zone (VZ), the germinal zone adjacent to the lateral ventricle and characteristically express the nuclear marker protein Pax635,36. They first expand by proliferative divisions37. With the onset of neurogenesis, APs start dividing asymmetrically, thereby generating BPs that accumulate in the subventricular zone (SVZ). The SVZ is the germinal zone basal to the VZ and constitutes the major site of neuron production in the developing dorsal telencephalon38,39,40,41,42. BPs consist of two major subtypes: basal intermediate progenitors and basal radial glia, with the latter sharing key features with APs including the expression of Pax641,43,44,45 and basal intermediate progenitors characteristically expressing the nuclear marker protein Tbr246,47. Newborn neurons migrate radially into the cortical plate (CP) in a birth date-dependent inside-out manner, in which later-born neurons migrate and settle past earlier-born neurons48,49,50.
Up to date, the host cells and alterations of T. gondii infection in the brain of human fetuses congenitally infected with T. gondii are still poorly understood, due to the difficulties in performing clinical studies in pregnant women. As such, whether T. gondii infects NPCs in the fetal brain and what the potential consequences on brain development are, remains currently unknown. The aim of this study is to determine the in vivo host cells of T. gondii and the developmental alterations associated with a congenital T. gondii infection in the fetal brain, specifically focusing on the neocortex. The study was conducted in the guinea pig, which represents a highly suitable animal model for human congenital toxoplasmosis, due to the similarities in brain maturity status at birth, in relative timing of cortical neurogenesis and in placentation to humans51,52,53. Here, we demonstrate that T. gondii infects NPCs, neurons and astrocytes in the fetal guinea pig brain following vertical transmission of the parasite. Our data show that T. gondii infection of the dam during first trimester of gestation results in massive changes in neocortex development of the fetus. Specifically, we observed a significant reduction in the number of neurons at end-neurogenesis and found a marked reduction in the number of BPs, specifically Pax6 and Tbr2-expressing BPs, in the fetal neocortex during mid-neurogenesis, indicating that impaired neurogenesis underlies the neuronal decrease in T. gondii infected fetuses. Moreover, we found T. gondii tachyzoites to be associated with microglia nodes in the fetal brain as early as second trimester of gestation.
Results
Fetuses were successfully infected with T. gondii 17 and 25 days after inoculation of dams
All guinea pig dams became pregnant upon first mating. No clinical abnormalities, i.e., in activity, movement, hair coat, water and food intake, breathing, mucosal color, urine, feces were detected in any of the dams during the daily assessment (Supplementary Table 1). Moreover, no abnormalities were found in the pregnant animals during the ultrasonographic and gynecological examination and no resorptions, abortions or stillbirth of fetuses were observed during the entire experiment. Litter size (mean ± SEM) of dams was 2.33 ± 0.29 for the control and 3.44 ± 0.34 for the infection groups.
Prior to infection, all blood samples of the control and infection groups were seronegative using immunoblotting against a T. gondii p30 surface antigen. In order to verify a T. gondii infection of the dam and fetus, tissue samples were obtained from distinct organs, i.e., maternal heart, liver, and spleen and fetal brain, heart, liver, spleen, thigh muscle, placenta and amniotic fluid, and analyzed for the presence of T. gondii DNA by qPCR targeting a T. gondii specific 529 base pair repeat element. In all dams and fetuses of the control groups, no T. gondii DNA was detected in any of the maternal and fetal tissues and organs analyzed (Supplementary Table 2, lines 43–74). In all dams of the infection groups, T. gondii DNA was detected in at least one maternal organ, indicating that all dams were successfully infected (Supplementary Table 2, lines 1, 6, 11, 14, 17, 22, 27, 32, 36). In all fetuses of dams dissected on gestation day 33, i.e., 10 days after inoculation of dams, no T. gondii DNA was detected in any of the tissues and organs analyzed (Supplementary Table 2, lines 2–5, 7–10, 12, 13). Thus, infection of fetuses dissected on gestation day 33 was considered as unsuccessful and the corresponding fetuses were excluded from further analysis. In all fetuses of dams dissected on gestation days 40 and 48, i.e., 17 and 25 days after inoculation of dams, T. gondii DNA was detected in at least two tissues and organs of each fetus, indicating their successful infection (Supplementary Table 2, lines 15, 16, 18–21, 23–25, 28–31, 33–35, 37–41).
T. gondii DNA was present in various fetal tissues and organs including the brain
Using qPCR analysis, T. gondii DNA was detected in all fetal placentas and in the majority of the fetal brain (89%), heart (78%) and spleen (67%) samples on gestation day 40 (Supplementary Table 2, line 26). By gestation day 48, the percentage of fetal tissues and organs containing T. gondii increased with its DNA being present in all fetal placental, amniotic fluid, brain and heart samples and in the majority of the fetal spleen (58%) and thigh muscle (78%) samples (Supplementary Table 2, line 42).
We next translated the Ct values obtained by qPCR into genomic equivalents of tachyzoites by interpolation from a parasite dilution curve and compared values from the same tissue or organ between different durations of infection, i.e., duration between inoculation of the dam and sampling of animals (Fig. 1). No significant differences were found between the T. gondii DNA loads of the intra-embryonic tissues and organs, i.e., brain, heart, lung, spleen and thigh muscle when different durations of infection were compared (Fig. 1a, b). However, T. gondii DNA load in the amniotic fluid was significantly higher in fetuses dissected on gestation day 48, i.e., 25 days after inoculation of dams, when compared with those infected for a shorter duration, i.e., dissected on gestation day 40, thus 17 days after inoculation of dams (Fig. 1a, b).
a, b T. gondii DNA loads in 10 mg tissue were obtained by qPCR in fetuses of dams inoculated with T. gondii on gestation day 23 and dissected on day 40 (a) and 48 (b). Center line, median; box limits, upper and lower quartiles; whiskers, 1.5× interquartile range; points, outliers. B brain, H heart, Lu lung, S spleen, M thigh muscle, P fetal placenta, A amniotic fluid. Solid lines indicate comparison of fetal tissues and organs obtained from dams infected for the same duration of infection. Dashed lines indicate comparison between the same tissue and organ within the different durations of infection. *P < 0.05; ***P < 0.001; ****P < 0.0001. Individual P values: comparison between tissues and organs on gestation day 40: P = 0.0433, P vs Lu; P = 0.0108, P vs M; P = 0.0002, P vs A; comparison between tissues and organs on gestation day 48: P = 0.0172 B vs S; P < 0.0001, P vs S, P < 0.0001, A vs S; P = 0.0001, P vs M; P = 0.0005, A vs M; comparison between gestation days 40 and 48: P < 0.0001, A. Only statistically significant differences are shown. Individual n values represent biologically independent samples: comparison between tissues and organs on gestation day 40: n = 9, B; n = 9, H; n = 5, Lu; n = 9, S; n = 9, M; n = 8, P; n = 9, A; comparison between tissues and organs on gestation day 48: n = 12, B; n = 11, H; n = 1, Lu; n = 11, S; n = 9, M; n = 11, P; n = 12, A.
When T. gondii DNA loads were compared between different tissues and organs within the same group of duration of infection, T. gondii DNA loads in fetuses dissected on gestation day 40 were significantly higher in the placenta than in the amniotic fluid and distinct intra-embryonic tissues and organs, i.e., thigh muscle and lung (Fig. 1a). Moreover, in fetuses dissected on gestation day 48, T. gondii DNA loads were significantly higher in the placenta and amniotic fluid than in the thigh muscle and spleen (Fig. 1b). No marked differences were found when T. gondii DNA loads were compared between the intra-embryonic tissues and organs, i.e., brain, heart, lung, spleen and muscle, on gestation day 40 (Fig. 1a). However, upon longer duration of infection, dissected on gestation day 48, i.e., 25 days after inoculation of dams, highest median T. gondii DNA loads in the fetus were observed in the brain being significantly higher when compared with the spleen (Fig. 1b).
The forebrain constitutes a main target region of T. gondii in the fetal brain
We next investigated, whether there is a specific target region of T. gondii within the guinea pig fetal brain. For this, we analyzed 5 randomly chosen sections per brain of T. gondii infected fetuses dissected on gestation days 40 and 48 by immunohistochemistry using an antibody for the T. gondii tachyzoite-specific surface antigen SAG154,55 and quantified delineated SAG1+ clusters (Fig. 2a). A SAG1+ cluster most likely represents a spatially delimited accumulation of T. gondii tachyzoites consisting of a primary tachyzoite, which initially invades the host cell, and its daughter cells, which arise from several cycles of endodyogeny7,56. We found T. gondii tachyzoite clusters to be present in one out of five (20%) brains of fetuses dissected on gestation day 40 and 4 out of 10 (40%) brains dissected on gestation day 48. When different brain regions, i.e., telencephalon, diencephalon, mesencephalon, metencephalon and myeloncephalon, were compared, all T. gondii tachyzoite clusters were located in the forebrain, i.e., telen- and diencephalon, with highest numbers being present in the neocortex (Fig. 2b). No T. gondii tachyzoite clusters were observed in brain regions caudal to the diencephalon (Fig. 2b). To verify the presence of T. gondii tissue cysts, we performed SAG1 immunohistochemistry together Dolichos biflorus agglutinin (DBA) staining on adjacent sections, in which T. gondii were detected by SAG1 immunohistochemistry (Supplementary Fig. 1). DBA binds to N-acetylgalactosamine moieties present on the T. gondii cyst wall57. T. gondii tissue cysts were solely detected in one section of a fetus dissected on gestation day 48. All cysts contained SAG1+ parasites, i.e., tachyzoites, thus indicating that they are at a very early stage of development.
a DAPI staining (blue) and immunofluorescence for SAG1 (red) on a 30 µm brain section of a guinea pig fetus of a dam inoculated with T. gondii on gestation day 23 and dissected on day 48. Open arrowheads indicate a SAG1+ T. gondii tachyzoite cluster. Scale bar, 10 µm. b Number of tachyzoite clusters detected by SAG1 immunofluorescence in the distinct brain regions of guinea pig fetuses of dams inoculated with T. gondii on gestation day 23 and dissected on days 40 and 48. Data are from all guinea pig fetal brains with Ct value below 35 as determined by qPCR for T. gondii (n = 5 biologically independent samples for gestation day 40, n = 10 biologically independent samples for gestation day 48, Supplementary Table 1). c Median section of an adult guinea pig brain. NC neocortex, LV lateral ventricle, BN basal nuclei, SA septal area, T thalamus, HT hypothalamus.
T. gondii infects neural progenitor cells, neurons, and astrocytes in the fetal forebrain
In a further step, we elucidated, which specific cell types are infected by T. gondii in the guinea pig fetal brain. To this end, we analyzed cortical sections of T. gondii infected fetuses dissected on gestation days 40 and 48 by double or triple immunohistochemistry using antibodies for SAG1 and one of the following cytoplasmic marker protein(s): (i) Nestin, an intermediate filament protein of NPCs58, (ii) MAP2, a microtubule-associated protein of neuronal dendrites and soma59, and neurofilament H, an intermediate filament protein of neuronal axons60,61, and (iii) GFAP, an intermediate filament protein of astrocytes62,63. Interestingly, T. gondii tachyzoites were completely encapsulated by Nestin+ immunofluorescence signal (Fig. 3a), thus revealing their presence in NPCs. Moreover, T. gondii tachyzoites were detected in neurons and astrocytes as visualized by the complete encapsulation of MAP2 and neurofilament H (Fig. 3b), and GFAP immunofluorescence signal, respectively (Fig. 3c). Together, this demonstrates the ability of T. gondii to infect NPCs, neurons as well as astrocytes in the fetal guinea pig brain following its vertical transmission.
a, b DAPI staining (blue) and immunofluorescence for Nestin (green, a), neurofilament H and MAP2 (green, b), or GFAP (green, c), and SAG1 (red) on 30 µm brain cryosections of guinea pig fetuses of dams inoculated with T. gondii on gestation day 23 and dissected on day 40 (b) or 48 (a, c). Image showing Nestin immunofluorescence represents a maximum intensity projection of 3 optical sections with a thickness of 0.2 µm each (a). Image showing MAP2 immunofluorescence represents a maximum intensity projection of 2 optical sections with a thickness of 0.2 µm each (b). Closed arrowheads indicate Nestin+ (a), neurofilament H/MAP2+ (b), or GFAP+ (c) cytoplasm. Open arrowheads indicate SAG1+ tachyzoites. 3D graphics were created by surface rendering for visualization only using Imaris. Scale bars, 10 µm.
T. gondii infection results in a decrease of neurons and NPC count in the fetal neocortex
To gain insight into the direct implications of the T. gondii infection in the guinea pig fetal neocortex, specifically on the pool size of the infected cells, we analyzed cortical sections at a medium position of the lateral ventricle per brain of the control and infection groups by immunohistochemistry using antibodies for characteristic marker proteins of the cells of interest. We first focused on neurons and used an antibody for the pan-neuronal marker Hu C/D (Fig. 4a–d)64,65. Quantification of Hu C/D+ cells revealed no significant differences in neuron number between fetuses of the control and the infection group dissected on gestation day 40 (Fig. 4a, b, e). However, on gestation day 48, the number of Hu C/D+ cells was significantly lower in the neocortex of fetuses infected with T. gondii when compared with those of the control group (Fig. 4c–e). No major differences in the distribution of Hu C/D+ cells between the control and infection groups on both gestation days were obvious, indicating that the apical-basal migration of neurons is not affected in the T. gondii infected brains.
a–d DAPI staining (blue) and immunofluorescence labeling for Hu C/D (red) on 30 µm brain cryosections of guinea pig fetuses of control dams (a, c) or dams inoculated with T. gondii on gestation day 23 (b, d) and dissected on day 40 (a, b) or 48 (c, d). The entire cortical wall is shown. CP, cortical plate. Scale bars, 50 µm. e Quantification of Hu C/D+ cells in the cortical wall, expressed as number of cells per 100 µm ventricular surface. Cortical wall corresponding to a total ventricular surface of 150–800 µm was analyzed. Center line, mean; error bar, SEM. Data of the infection groups are from all guinea pig brains with Ct value below 35 as determined by qPCR for T. gondii (n = 5 for gestation day 40, n = 10 biologically independent samples for gestation day 48, Supplementary Table 1). Data of the control group are as follows: n = 7 biologically independent samples for gestation day 40, n = 5 biologically independent samples for gestation day 48. *P < 0.05 (P = 0.0181, df = 13).
We next analyzed cortical sections by double immunohistochemistry using antibodies for distinct NPC markers, i.e., Pax6, a transcription factor characteristically expressed by APs and basal radial glia, and Tbr2, a transcription factor characteristically expressed by basal intermediate progenitors (Fig. 5a, b)41,43,44,46. As shown previously66, no Tbr2+ cells were detected in the neocortex of the control and infected groups on gestation day 48, indicating that cortical neurogenesis in the guinea pig has terminated before (Supplementary Fig. 2). On gestation day 40, which constitutes mid-neurogenesis in the guinea pig neocortex66, no significant differences in the number of Pax6+ and/or Tbr2+ cells of the VZ between the control and infected fetuses were detected (Fig. 5c), indicating that the pool size of the primary NPCs, i.e., APs, is largely unaffected in the developing neocortex of fetuses infected with T. gondii when compared with that of controls. We then focused our analysis on the secondary NPCs in the SVZ/IZ, i.e., BPs. Interestingly, their total number, i.e., the sum of Pax6+/Tbr2–, Pax6+/Tbr2+, Pax6−/Tbr2+ NPCs, on gestation day 40 was significantly lower in T. gondii infected fetuses when compared with that of controls (Fig. 5d). When investigating whether this reduction was attributable to a specific BP subpopulation, we found the number of Pax6+/Tbr2+ BPs to be significantly decreased in T. gondii infected fetuses when compared with controls (Fig. 5d). Together, our data show that T. gondii infection of NPCs and neurons in the fetal guinea pig neocortex impacts their number, resulting in a reduction of the NPC pool during mid-neurogenesis and that of neurons at end-neurogenesis. No significant differences were observed when the cortical thickness was compared between the control and infection group of both gestation days (Supplementary Fig. 3). Together, this suggests that the reduced cell numbers lead to a decrease in cell density but not to a decrease in cortical wall thickness in the brain of T. gondii infected fetuses.
a, b DAPI staining (blue) and immunofluorescence labeling for Pax6 (red) and Tbr2 (green) on 30 µm brain cryosections of guinea pig fetuses of control dams (a) or dams inoculated with T. gondii on gestation day 23 (b) and dissected on day 40. Scale bar, 50 µm. c, d Quantification of Pax6+ (red) and/or Tbr2+ (green) NPCs in the ventricular zone (VZ, c) and subventricular zone/intermediate zone (SVZ/IZ), d), expressed as number of cells per 100 µm ventricular surface. Cortical wall corresponding to a total ventricular surface of 230–500 µm was analyzed. The dashed line indicates the border between VZ and SVZ/IZ. Center line, mean; error bar, SEM. Data of the infection groups are from all guinea pig brains with Ct value below 35 as determined by qPCR for T. gondii (n = 5 for gestation day 40, biologically independent samples, Supplementary Table 1). Control group: n = 7 biologically independent samples for gestation day 40. *P < 0.05 (P = 0.0440, df = 10, NPCs, i.e., the sum of Pax6+/Tbr2–, Pax6+/Tbr2+, Pax6–/Tbr2+ cells, in SVZ/IZ; P = 0.0441, df = 10, Pax6+/Tbr2+ cells in SVZ/IZ).
In a final step, we focused on astrocytes and analyzed cortical sections by immunohistochemistry using an antibody for GFAP (Fig. 6a, b). Similar to previous observations66, mature astrocytes, which exhibit a typical star-shaped appearance, were first detected after the end of neurogenesis, i.e., on gestation day 48 in the guinea pig neocortex (Fig. 6a, b). We then quantified the GFAP immunofluorescence intensity in the control and infected fetuses obtained on gestation day 48 and found no difference when the two groups were compared (Fig. 6c). This indicates that T. gondii infection of the fetal guinea pig neocortex does not affect the number of astrocytes.
a, b DAPI staining (blue) and immunofluorescence for GFAP (green) on 30 µm brain cryosections of guinea pig fetuses of control (a) or infected (b) dams dissected on gestation day 48. Dams were inoculated with T. gondii on gestation day 23. Scale bar, 50 µm. The entire cortical wall is shown. CP, cortical plate. Scale bars, 50 µm. c Quantification of GFAP+ labeling intensity in the cortical wall, expressed as number of voxels per 100 µm ventricular surface. Cortical wall corresponding to a total ventricular surface of 150–250 µm was analyzed. Center line, mean; error bar, SEM. Data of the infection groups are from all guinea pig brains with Ct value below 35 as determined by qPCR for T. gondii (n = 10 biologically independent samples, for gestation day 48, Supplementary Table 1). Data of the control group are as follows: n = 5 biologically independent samples. (P = 0.3325, df = 13).
T. gondii infection of the fetal neocortex is not associated with an increase in cell death
Previous studies demonstrated the ability of T. gondii to induce cell death67,68,69. In order to investigate whether cell death accounts for the observed NPC and neuron loss in the T. gondii infected guinea pig neocortex, we analyzed cortical sections of the control and infection groups by immunohistochemistry using an antibody for caspase-3, a marker of programmed cell death (Supplementary Fig. 4)70,71. Only a few apoptotic cells were detected in the cortical wall of the control group at both stages analyzed (Table 1). Similarly, the number of apoptotic cells in the cortical wall of fetuses dissected on gestation days 40 and 48 was markedly low (Table 1). No significant difference in their number was detected when the control and infection groups were compared (Table 1). Moreover, we analyzed DAPI-stained nuclei for pyknosis and/or karyorrhexis, which are hallmarks of cell death, in the cortical wall of the neocortex of both infection groups. We found all pyknotic and fragmented nuclei to be present in caspase-3+ cells. Together, this suggests that cell death is unlikely to account for the reduction in NPC and neuron count observed in the neocortex of T. gondii infected fetuses.
Focal microglioses are present in the brain of T. gondii infected fetuses
In the following, we aimed to gain insight into the fetal immune response against T. gondii in the guinea pig neocortex, focusing on microglia, which represent the resident immune cells in the central nervous system first72,73. For this, the adjacent section of the brain section in which T. gondii tachyzoites were detected and a control section of a corresponding brain area of fetuses dissected on gestation days 40 and 48 were stained with antibodies for Iba1, a characteristic marker of microglia74,75 and SAG1 (Fig. 7). In fetuses of the control group, microglia were present in the neocortex as early as gestation day 40, i.e., during mid-neurogenesis (Fig. 7a). Remarkably, in the brain of guinea pig fetuses of both infection groups, all T. gondii tachyzoites were found in the center of the microglia aggregations and microglia nodules were only present in association with tachyzoites (Fig. 7c, d). Quantification of Iba1 immunofluorescence intensity in the tachyzoite related lesions and corresponding brain areas of the control group revealed a significant increase in the Iba1 fluorescence labeling intensity in the brain of T. gondii infected fetuses (Fig. 7e). This suggests that parasitic lesions are associated with focal or multifocal microglioses in the brain of guinea pig fetuses 17 days after inoculation of dams with T. gondii.
a–c DAPI staining (blue) and immunofluorescence for Iba1 (green) and SAG1 (red) on 30 µm brain cryosections of guinea pig fetuses of control dams dissected on gestation days 40 (a) or 48 (b) and dams inoculated with T. gondii on gestation day 23 and dissected on day 40 (c, d). Scale bar, 50 µm. Arrowheads indicate Iba1+ microglia. Arrows indicate SAG1+ T. gondii tachyzoites. Dashed line outlines an agglomeration of Iba1+ microglia surrounding SAG1+ T. gondii tachyzoites. Image in (d) shows the same section and brain region as in (c) without the presence of tachyzoites. e Quantification of Iba1 labeling intensity as detected by immunofluorescence labeling for Iba1. Labeling intensities were quantified in a 200 × 200 µm area including a tachyzoite cluster of guinea pig fetuses of dams inoculated with T. gondii on gestation day 23 and from a 200 × 200 µm area covering the same brain region of control fetuses, dissected on gestation days 40 and 48. Results were expressed as voxels per µm2. Center line, mean; error bar, SEM. Data are from 15 T. gondii tachyzoite clusters observed in 5 fetuses dissected on gestation days 40 and 48 (Fig. 2) and the corresponding regions of the control groups. **P < 0.01 (P = 0.0064, df = 28, n = 15 biologically independent samples). Dots not displayed for the infected group: 4.01, 2.52, 4.62.
During activation in response to various stimuli, e.g., brain infection, microglia undergo distinct morphological changes. Non-activated microglia mainly exhibit a ramified morphology, whereas fully activated microglia acquire an amoeboid shape76. In order to analyze whether T. gondii infection is associated with a change in microglia morphology in the fetal brain, microglia in the tachyzoite related lesions and corresponding brain areas of the control group of fetuses dissected on gestation days 40 and 48 were classified as activated and non-activated using Imaris surface classification (Supplementary Fig. 5). This revealed that tachyzoite related lesions contain a higher proportion of amoeboid to ramified microglia than corresponding control areas. Together, this indicates that a fetal immune response against T. gondii associated with the presence of formation of activated microglia nodules is established in the brain of T. gondii infected fetuses as early as gestation day 40.
Secondary to microglia, astroglia may be recruited to the site of inflammation in the brain77. In order to analyze whether astrocytes contribute to the immune response in foci of T. gondii tachyzoites, we analyzed the adjacent section of the brain section, in which T. gondii tachyzoites were detected on gestation day 48, by immunohistochemistry for GFAP (Fig. 8a, b). Quantification of the GFAP labeling intensity in the tachyzoite related lesions and corresponding brain areas of the control group revealed no significant difference between the control and infection group (Fig. 8c). This indicates that parasitic lesions are not associated with focal or multifocal astroglioses in the brain of guinea pig fetuses 25 days after inoculation of dams with T. gondii.
a, b DAPI staining (blue) and immunofluorescence for GFAP (green) and SAG1 (red) on 30 µm brain cryosections of guinea pig fetuses of control (a) or infected (b) dams dissected on gestation day 48. Dams were inoculated with T. gondii on gestation day 23. Scale bar, 50 µm. Arrowheads indicate GFAP+ astroglia. Arrows indicate SAG1+ T. gondii tachyzoites. c Quantification of GFAP labeling intensity as detected by immunofluorescence labeling for GFAP. Intensities were quantified in a 200 × 200 µm area including a tachyzoite cluster of guinea pig fetuses of dams inoculated with T. gondii on gestation day 23 and from a 200 × 200 µm area covering the same brain region of control fetuses, dissected on days 40 and 48. Results were expressed as voxels per µm². Center line, mean; error bar, SEM. Data are from 15 T. gondii tachyzoite clusters observed in 5 fetuses dissected on gestation days 40 and 48 (Fig. 2) and the corresponding regions of the control groups. (P = 0.4688, df = 28, n = 15 biologically independent samples). Dots not displayed for the control group: 3.54, 2.52, and for the infected group: 2.51.
Discussion
This project provides novel and fundamental contributions to the understanding of the pathogenesis of congenital toxoplasmosis, specifically in the context of neocortex development and alterations of fetuses infected with T. gondii. We have previously established the guinea pig as a highly suitable animal model for human congenital toxoplasmosis in an attempt to overcome difficulties in performing clinical studies in pregnant women and in evaluating work in cell and tissue culture systems that fail to re-capitulate the complexity of a living animal53. Since all dams survived and no resorptions, abortions or stillbirth of fetuses were observed during the entire trial, our data confirm that oral administration of 100 T. gondii oocysts of the ME49 strain in the beginning of the second trimester of gestation, i.e., on gestation day 23, has no major impact on the guinea pig dam and offspring survival rate53. Moreover, we show that the administration of T. gondii oocysts to the dams has no negative effect on litter size.
We found no T. gondii DNA in the wide range of tissues and organs investigated, i.e., brain, heart, liver, lung, spleen, muscle, placenta and amniotic fluid, of fetuses dissected on gestation day 33, indicating that 10 days are not sufficient for a congenital transmission of the parasite and subsequent infection of the guinea pig fetus. When fetuses dissected on gestation days 40 and 48 were analyzed, T. gondii DNA was in two or more tissues or organs of each fetus, revealing that the parasite is stably transmitted to a larger extent to and replicates in the fetus 17 and 25 days after oral inoculation of the dam. These data are in line with a former study52, in which pregnant guinea pigs were orally inoculated with 100 tissue cysts of the 76 K strain. We previously observed that the duration a pregnant dam is infected affects the T. gondii load in the guinea pig offspring53. Indeed, this study shows that longer duration of T. gondii infection results in higher T. gondii DNA load in the extra-embryonic amniotic fluid. However, no differences in T. gondii DNA load were observed within the intra-embryonic tissues and organs. Given that in our previous study53, the duration of T. gondii incubation was up to 51 days, we suppose that the timespan, i.e., 8 days, between the two infection groups analyzed in this study was simply not long enough for any significant changes in the T. gondii DNA loads of the fetal tissues and organs to occur. Upon infection for 17 days, we observed no significant differences in the T. gondii DNA load between any of the fetal tissues and organs analyzed, which is consistent with previously published data53. Interestingly, when animals were analyzed after 25 days of inoculation, highest median T. gondii DNA loads in the fetus were observed in the brain. Moreover, the fetal brain possesses a remarkably high T. gondii positivity rate in both infection groups analyzed. Together, this confirms that the brain constitutes a preferred host organ of T. gondii in mammals including human52,53,78,79,80,81,82.
All T. gondii tachyzoites were located in the forebrain of guinea pig fetuses, mostly in the telencephalic basal nuclei and neocortex, which is in line with published data obtained in postnatal mammals including mice and human showing high T. gondii cyst burden to be present in the telencephalon including the amygdala, hippocampus, and various parts of the pallium such as the entorhinal, somatosensory, motor, orbital, frontal association, and visual cortex83,84,85. Moreover, we found T. gondii tachyzoites to be present in the choroid plexus and the lateral ventricle, thus providing further evidence for the notion that translocation across the choroid plexus and cerebrospinal fluid is a means for T. gondii to enter the brain86,87.
This study provides important new data on the in vivo host cells of T. gondii in the offspring neocortex before birth. Similar to in vivo data in the adult brain demonstrating that neurons and astrocytes represent targets of T. gondii, we observed T. gondii to infect neurons and astrocytes in the brain of guinea pig fetuses following the parasite’s vertical transmission10,24,88,89. In this regard it is of great importance that NPCs are almost exclusively present in high abundance in the prenatal neocortex29,30,31,32,33,34,66. Indeed, this study reveals that T. gondii infects NPCs in the brain of guinea pig fetuses congenitally infected with the parasite. These data are consistent with in vitro studies using a primary murine NPC culture90,91. As a result of congenital infection, we found the total number of BPs, which are known to generate the majority of cortical neurons38,39,40,41,42, to be markedly reduced in the neocortex of guinea pig fetuses during mid-neurogenesis. Specifically, we found the reduction in BP number to be mainly attributed to the Pax6+/Tbr2+ BP subtype population. On the assumption that sustained Pax6 expression in NPCs is linked to higher cell proliferation42,92, our data suggest that proliferative BPs committed to the neuronal lineage are most affected by T. gondii infection. As delaying the switch of symmetric proliferative NPC divisions to asymmetric neurogenic NPC divisions results in an exponential accumulation of neurons over time93, one would assume that the impact of reduced BP proliferation on neuron count manifests during final stages of neurogenesis. Indeed, our data reveal that the number of neurons is significantly reduced in the neocortex of fetuses infected with T. gondii on gestation 48, i.e., at end-neurogenesis when compared to healthy controls. These data confirm previous studies in children showing prenatal infection with T. gondii is associated with microcephaly6,20. Importantly, given that the reduction in neuron number is not primarily linked to an increase in neuronal cell death, our findings also indicate that, instead of neuron loss, impaired neurogenesis may underlie the reduction in neuron number observed in the neocortex of offspring congenitally infected with T. gondii.
Again, the reduction in BP cell counts observed in the neocortex of T. gondii infected fetuses was not associated with an increase in their cell death. Similarly, in vitro data using a primary murine NPC culture showed that an infection by the ME49 strain of T. gondii results in reduced NPC proliferation with no apoptosis induction91. In this regard it is interesting to note that T. gondii infection has been shown to result in dysregulation of the host cell cycle, specifically to arrest host cell cycle before progression to mitosis22,25,94. Moreover, recent data indicate that T. gondii induces a M cell cycle arrest by propagating chromosome segregation errors, mitotic spindle alteration and blockage of cytokinesis progression in primary bovine endothelial cells27. Therefore, one possible scenario might be that alterations in the BP cell cycle progression, specifically a blockage of its cell division rate, may explain the decrease in neurogenesis of the neocortex of T. gondii infected fetuses. Interestingly, T. gondii is able to inject effector proteins, e.g., rhoptry proteins, into cells it does not invade with the injected cells exceeding the infected cells many times over95. In this regard it is interesting to note, that T. gondii rhoptry protein ROP16 has been found to partially mediate cell cycle arrest in a human neuroblastoma cell line96. Hence, it could be assumed that T. gondii invasion and secretion of T. gondii effector proteins into distinct NPCs collectively subvert their functions leading to a global reduction in neurogenesis in infected fetuses. As an additional explanation, indirect environmental effects from the host response, e.g., from microglia may contribute to the observed reduction of the BP cell pool. Future studies will focus on the cellular and molecular alterations including the mode and rate of cell division of NPCs in the fetal brain induced by T. gondii as well as the specific molecular mechanisms that play a role in parasite invasion, proliferation, clearing of cells and injection of effector proteins in the fetal brain. To precisely determine T. gondii cell tropism in the fetal brain, highly sensitive methods, e.g., flow cytometry, should be used to complement the data provided by this study.
Moreover, our data indicate that congenital T. gondii infection does not affect the number of astrocytes in the fetal guinea pig brain, thus confirming the results of a recent in vitro study using a primary murine NPC culture, in which no alterations in the number of astrocytes were observed upon T. gondii infection90. NPCs are known to generate glial cells including astrocytes at later stages of cortical development once neurogenesis is mostly complete97,98. As we found no alteration in the number of Pax6+/Tbr2− NPC BPs, which are not committed to the neuronal lineage, it is very likely that the generation of astrocytes—contrary to that of neurons—by NCPs is not affected in the neocortex of guinea pig fetuses upon vertical T. gondii transmission, which in turn implies that distinct NPC subtypes differ in their susceptibility to T. gondii infection. However, as astrocytes—in contrast to neurons—maintain the ability to self-renew99,100, it cannot be ruled out that a decrease in astrocyte generation by NPCs was compensated by increased in astrocyte proliferation, leading to recovery of their quantity.
After birth, T. gondii infection of the central nervous system triggers an immune response by microglia, the resident immune cells of the brain and spinal cord, during the acute phase of infection13,101. We previously observed focal or multifocal microglioses in the neocortex of newborn guinea pigs prenatally infected with T. gondii53. During prenatal development, microglia start to colonize the brain concurrently with neurogenesis and prior to the generation of other glial cells102,103,104,105. As such, they might play various roles and are involved in neurogenesis, gliogenesis, and neuronal circuit formation106. Here, we show that the fetal guinea pig neocortex is populated by microglia as early as day 40 of gestation, i.e., during mid-neurogenesis. We found that congenital T. gondii infection results in the formation of activated microglia nodules in the guinea pig fetal brain in the second and third trimester of gestation, i.e., on gestation days 40 and 48, which suggests that microglia generate immune responses, specifically contributing to host defense of the brain against T. gondii, long before birth. Microglia are able to induce the activation of astrocytes, which may act as immunocompetent cells by secreting inflammatory cytokines and producing reactive oxygen species77,107. Indeed, previous data showed activated astrocytes to be associated with foci of microglia containing T. gondii tachyzoite clusters in the adult murine cortex following reactivation of chronic brain infection108. However, in this study no signs of focal astrogliosis associated with T. gondii tachyzoite clusters in the guinea pig brain were observed on gestation day 48. Given the time span of 25 days between inoculation of dams and analysis of the fetal brain, it is likely that this time window is too short for astrocytes to become activated to a large extent. Therefore, future studies using longer incubation periods and specific markers of astrocyte activation will reveal whether astrocytes - in addition to microglia - are part of the host defense against T. gondii in the fetal brain following congenital infection.
In summary, our data reveal that the neocortex is a major target region of T. gondii in fetuses of congenitally infected guinea pigs. We show for the first time that T. gondii infects NPCs, neurons and astrocytes in the fetal brain. Our results indicate that the reduction in neuron numbers observed in the neocortex of offspring congenitally infected with T. gondii is associated with its reduced generation and that microglia activation and recruitment to T. gondii tachyzoites is already established during the period of mid-neurogenesis. Together, our findings contribute considerably to the understanding of the cortical malformations observed in individuals congenitally infected with T. gondii and help to establish new treatments and solutions for congenital toxoplasmosis.
Methods
Ethics and animal welfare approval
All animal experiments were performed in accordance with German animal welfare legislation. The guinea pig study was approved by the Landesdirektion Sachsen (TVV 45/17, DD24.1-5131./390/47) and infection of cats to provide oocyst infection material was permitted by the ethics commission of the Animal Care and Use Committee of the German Lower Saxony State Office for Consumer Protection and Food Safety (reference number 33.19-42502-05-17A206). We have complied with all relevant ethical regulations for animal testing.
Animals
Female Dunkin Hartley guinea pigs (n = 18, aged 3–6 months) were obtained from Charles River Laboratories (Ecully, France) and housed in the animal-care facility of the Institute of Parasitology, Faculty of Veterinary Medicine, University of Leipzig, Leipzig, Germany under previously described conditions53. In brief, dams were kept in groups of two in 50 × 70 × 50 cm wire mesh cages and provided water supplemented with 400 mg/l ascorbic acid, standard diet pellets (Altromin Spezialfutter, Lage, Germany) and fresh vegetables ad libitum. Room temperature was maintained at 19–25 °C and relative humidity at 55% (±10%). Light and dark cycle was set to 12:12 h. All dams were assessed daily based on a scoring system (Supplementary Table 1) during the entire trial.
Mating and pregnancy examination
Dams were mated at the animal-care facility of the Institute of Parasitology, Faculty of Veterinary Medicine, University of Leipzig, Germany. Before, their sexual cycle was synchronized by oral administration of Altrenogest (Regumate® Equine 2,2 mg/ml, MSD Tiergesundheit, Unterschleißheim, Germany) at 0.22 mg/kg body weight once a day for 15 days53. Natural mating was initiated 2 days after the end of treatment by housing four females with one breeding ram for 4 days. Successful pregnancy was examined by ultrasound scan using GE Logiq 400 CL (pet mode, 7–10 MHz sample, GE Healthcare, Solingen, Germany). The day of successful mating is considered as gestation day 0 ± 253. During ultrasound scan, the reproductive system, i.e., ovary and uterus wall, of all dams was examined.
Serological investigation
Blood samples of all dams were collected from the Vena saphena lateralis immediately before infection and centrifuged (2500 × g, 10 min, 4 °C). Serum was analyzed by immunoblotting against T. gondii surface antigen p30 (SAG1) as previously described109, but using a peroxidase conjugated anti-guinea pig IgG (H + L, Jackson Immunoresearch Laboratories, West Grove, USA) instead of a peroxidase conjugated anti-mouse IgG.
Infection
T. gondii oocysts (Strain ME49) were provided by the Institute of Parasitology, University of Veterinary Medicine Hannover, Germany. Oocysts were generated as previously described53. In brief, seronegative cats were given meat supplemented with brain, muscle, liver and spleen of guinea pigs chronically infected with T. gondii. Cat feces were purified using a sucrose solution gradient. Isolated oocysts were stored in 2% sulfuric acid at 4 °C for 1.5–2.5 months. Immediately before infection, 1 M sodium hydroxide solution was added to the oocyst suspension. Sporulated oocysts were quantified using a Neubauer-Improved cell counting chamber (Paul Marienfeld, Lauda-Königshofen, Germany). Oocysts were suspended in 500 µl phosphate buffered saline (PBS) and administered orally with a 16 G buttoned cannula (Henry Schein Dental, Langen, Germany). Guinea pigs were randomly divided into a control (n = 9) and infection (n = 9) group. Dams of the infection group were administrated 100 oocysts on gestation day 23. Dams of the control group received 500 µl PBS solution only.
Euthanasia and dissection
Three dams and their corresponding litters of the control and infection group were euthanized by intraperitoneal injection of 500 mg/kg pentobarbital sodium on gestation days 33, 40 and 48, respectively. Fetuses were carefully dissected, and tissue samples were obtained from fetal brain, heart, liver, spleen, quadriceps femoris muscle, fetal placenta and amniotic fluid. Up to 600 mg of tissue was sampled per location. In case the entire tissue or organ weighed more, samples were taken randomly from at least 4 different regions. Except for the brain, the entire tissue and organ samples were frozen at −80 °C until further processing. Immediately after the removal of the brain, the cerebral hemispheres were separated. One cerebral hemisphere was frozen at −80 °C and used for qPCR. The other cerebral hemisphere was fixed in 4% paraformaldehyde for 4 days, stored in PBS at 4 °C and used for immunohistochemistry.
Tissue homogenization and DNA extraction
Fetal tissue samples were processed using NucleoMag-Tissue kit (Macherey-Nagel, Düren, Germany) according to the manufacturer´s instructions with the following modifications: tissue samples (up to 600 mg) were incubated with lysis buffer (T1) supplied with the NucleoMag-Tissue kit (Macherey-Nagel, Düren, Germany) at ratio 1:2 and two stainless steel balls (diameter 6 mm, TIS Wälzkörpertechnologie, Gauting, Germany) were added. The sample solution was homogenized using a TissueLyser II (Qiagen, Hilden, Germany) at 3000 Hz for 60 s. Next, proteinase K of the NucleoMag-Tissue kit was added to the sample solution at ratio 1:10 and the solution was incubated at 56 °C overnight. 220 µl of lysate, corresponding to 100 mg of starting material, was used for all further extraction steps that were carried out using a King Fisher Flex resulting in 100 µl purified DNA (ThermoScientific, Waltham, USA).
Quantitative PCR
A probe-based qPCR was applied, in which the 529 bp repeat element, characterized by high specificity and sensitivity for detection of T. gondii, was used as a sequence110,111. For all tissue and organ samples, qPCR was carried out as follows: primers and probes (MWG-Biotech, Ebersberg, Germany) were applied as previously described112 according to the assay protocol “Toxo529REP PCR” (Supplementary Table 3)53. An internal control according to113 was used for inhibition detection as previously described (Supplementary Table 3)53,114. When a negative result was due to PCR inhibition, the respective data was excluded from the data analysis. qPCR reactions were carried out in a CFX96 cycler (Biorad Laboratories, Kabelsketal, Germany) using 10 µl of purified DNA and the PerfeCTa MultiPlex qPCR ToughMix (VWR International, Dresden, Germany). qPCR conditions were as follows: 2 min at 50 °C and 10 min at 95 °C (initial denaturation). This was followed by 55 cycles, each consisting of 15 s at 95 °C (denaturation) and 1 min at 60 °C (hybridization and elongation). All qPCR results were evaluated using the CFX manager software version 1.6 (Biorad Laboratories, Kabelsketal, Germany). PCR results with a quantification cycle (Ct) equal to or higher than 40 were stated as Ct = 40 and considered as negative53. Brains of fetuses, whose Ct value was below 35 were included in the immunohistochemistry analysis. To establish a standard curve, tachyzoites were extracted from cell culture under the same conditions. Different negative extracts (guinea pig brain and muscle) were used for a 10-fold dilution series (2.8 × 101–2.8 × 105) in quintuplicates. The parameters for this semi-logarithmic standard curve are as follows: y = −3.406x + 36.36, R2 = 0.9977, E = 96.6%. Using this curve, Ct values were translated into genomic equivalents of tachyzoites.
Immunocytochemistry
Cerebral hemispheres were processed and subjected to an immunohistochemistry protocol as described previously115. In brief, fixed hemispheres were dehydrated in 30% sucrose in PBS at room temperature, embedded in Tissue-Tek (Sakura Finetek, Staufen im Breisgau, Germany) and stored at −20 °C. Sections were cut at 30 μm using a Leica cryoystat (Leica CM1850, Leica Biosystems, Wetzlar, Germany) and stored at −20 °C. Complete brain was cut coronally.
For analysis of regional tropism of T. gondii tachyzoites, five randomly chosen sections per brain of all fetuses with Ct value below 35 were used. For analysis of T. gondii host cells, 6–8 sections per brain in close proximity to the section, in which T. gondii tachyzoites observed, were analyzed. For quantification of neurons, NPCs, apoptosis and astrocytes in the neocortex, the section at a medium position of the lateral ventricle with regard to the rostro-caudal axis per brain of all fetuses with Ct value below 35 was used. For analysis of focal micro- and astrogliosis, the adjacent section, to which T. gondii tachyzoites were observed, was evaluated.
Sections for Pax6, Tbr2 and Hu C/D immunohistochemistry were subjected to an antigen retrieval protocol by heating sections for 1 h at 90 °C in 0.01 M citrate buffer (pH 6). All sections were permeabilized with 0.3% Triton X-100 in PBS and quenched with 0.1 M glycine. Antibodies were diluted in 0.2% gelatine-PBS. Primary antibodies were incubated overnight at 4 °C and secondary antibodies were incubated for 1 h at room temperature. The following primary antibodies were used: Pax6 (1:200, rabbit, Biolegend, London, United Kingdom, 901301), Tbr2 (1:200, sheep, R&D Systems, Abingdon, United Kingdom, AF6166), Hu C/D (1:500, rabbit, Abcam, Amsterdam, Netherlands, ab184267), neurofilament H (1:500, chicken, Abcam, Amsterdam, Netherlands, ab8135), SAG1 (1:1200, mouse, Bio-Rad Laboratories, Feldkirchen, Germany, 9070-2020), MAP2 (1:1000, chicken, Abcam, Amsterdam, Netherlands, ab5392), GFAP (1:500, rabbit, antibodies.com, Cambridge, United Kingdom, A85419), caspase 3 (1:400, rabbit, Sigma-Aldrich Chemie, Steinheim, Germany, C8487) and IBA1 (1:500, rabbit, SynapticSystems, Göttingen, Germany, 234003). Pax6, Tbr2, Hu C/D, neurofilament H, MAP2 and GFAP antibodies have previously been successfully used in the immunohistochemistry analysis of fetal guinea pig brain tissue66. Dolichos biflorus agglutinin FITC-conjugated were obtained from Biozol (1:200, Eching, Germany, VEC-FL-1031- 5). Donkey secondary antibodies coupled to Alexa Fluor® 488 chicken (A11039), mouse (A21202), and rat (A21208), Alexa Fluor® 555 mouse (A31570) and rabbit (A31572), Alexa Fluor® 647 sheep (A21448) (1:500, Invitrogen, Darmstadt, Germany) and Alexa Fluor® 647 chicken (703-606-155) (1:500, Jackson ImmunoResearch Europe, Ely, UK) were used. All sections were counterstained with DAPI (1:500, Sigma, Taufkirchen, Germany), mounted in Mowiol (Merck Biosciences, Darmstadt, Germany), coverslipped and kept at 4 °C.
Confocal laser scanning microscopy and deconvolution
Brain sections were imaged with a confocal laser scanning microscope (CLSM) Leica TCS SP8 (Leica Microsystems, Mannheim, Germany), using the software Leica Application Suite X (LAS-X 3.5.7). Images were acquired using the following microscope settings: bidirectional scan, scan speed 600 Hz, pinhole 1 Airy unit, and 3x line averaging. Sequential scanning of each channel separately was used to minimize cross talk between applied dyes. DAPI was excited at 405 nm (PMT detection range: 493–541 nm), Alexa Fluor® 488 at 488 nm (PMT detection range 493–541 nm), Alexa Fluor® 555 at 561 nm (HyD detection range 565–618 nm), and Alexa Fluor® 647 at 633 nm (HyD detection range 648–699 nm). The transmission (attenuator value) of each laser line was set so that the signal (8 bit-encoding) was just above saturation.
For analysis of regional tropism of T. gondii tachyzoites, tachyzoite clusters were manually determined under transmitted light using a ×40/1.10 W objective. For analysis of T. gondii host cells, a ×63/1.2 W objective was used and a scan resolution equivalent to a voxel size of 69 × 69 × 356 nm. Image stacks consisting of up to 61 layers were recorded to ensure that the entire parasite and compartment of the infected host cell was completely included. For quantification of neurons, NPCs and apoptosis, and of Iba1 and GFAP labeling intensity, a ×40/1.10 W objective was used and a scan resolution equivalent to a voxel size of 75 × 75 × 200 nm. Tile scans were recorded as z-stacks consisting of up to 5 layers.
Deconvolution of CLSM images, using Huygens Professional, version 20.10 (SVI, Hilversum, The Netherlands), was applied to reduce optical aberrations and to correct for the discrepancy in refractive indices (IR) of the embedding (IR = 1.49) and immersion media (IR = 1.33). Microscopic parameters were set according to the image metadata. A theoretical point spread function was used, and the following deconvolution parameters were set for batch processing with the Classic Maximum Likelihood Estimation (CMLE) algorithm: maximum iterations = 40, quality change threshold = 0.01, signal-to-noise ratio = 6.6667. Background for images of T. gondii host cell analysis and quantification of apoptosis and Iba1 and GFAP labeling intensity, all channels = 0. Background for images of quantification of neurons and NPCs: DAPI = 10.5, Alexa Fluor® 488 = 12, Alexa Fluor® 647 = 8.
Data analysis
The ventricular zone (VZ), subventricular zone (SVZ), intermediate zone (IZ) and cortical plate (CP) were identified based on their cytoarchitecture and, in case of the SVZ, based on the presence and abundance of Tbr2 positive nuclei. In brief, the VZ represents a densely packed cell layer lining the lateral ventricle and whose nuclei exhibit radial morphology. The SVZ is located basally to the VZ and exhibits a looser and sparser cell arrangement than the VZ. The apical border of the SVZ is marked by the presence of a continuous Tbr2 positive nuclear layer.
The IZ contains very low cell density and lies between the SVZ and the CP. The CP is a cell layer adjacent to the IZ, which represents a high cell density and radially aligned nuclei.
Imaris 9.7.2 (Oxford Instruments, Abingdon, UK) was used for image analysis. For quantification of neurons, NPCs and apoptosis, and of Iba1 and GFAP labeling intensity, only the middle layer of the z-stacks was used.
For quantification of neurons and NPCs, colocalization between channels for DAPI and Hu C/D, DAPI and Pax6, DAPI and Tbr2, DAPI and Pax6 and Tbr2 was displayed. Intensity thresholds for corresponding channels were set as follows: DAPI = 10.5, Hu C/D = 9, Pax6 and Tbr2 = 13 each. The segmentation of colocalized signals was achieved by the following settings: surface detail = 0.2 μm, thresholding: background subtraction, diameters of largest sphere = 6 μm, manual threshold value: DAPI and Hu C/D = 2, DAPI and Pax6 = 8, DAPI and Tbr2 = 8, DAPI and Pax6 and Tbr2 = 4.5, seed point diameter = 6 μm, quality: DAPI and Hu C/D > 1, DAPI and Pax6 > 2, DAPI and Tbr2 > 2, DAPI and Pax6 and Tbr2 > 1.8. If nuclei of individual cells were displayed as merged objects by automatic segmentation, these objects were separated manually. The number of cells was quantified in a rectangle spanning the corresponding cortical zone with an apical edge length of 100 µm.
For astrocyte analysis in the neocortex, the number of voxels representing GFAP labeling with intensities greater than 50 out of 255 (8-bit coding) was quantified in a rectangle spanning entire cortical wall with an apical edge length of 100 µm. Apoptotic cells were quantified in a rectangle spanning the entire cortical wall with an apical edge length of 100 µm. Cells with a caspase-3 fluorescence intensity of more than 50 out of 255 (8-bit coding) and nuclear changes (e.g., segmentations) detected in the DAPI signal were considered as positive (Supplementary Fig. 4). For analysis of focal micro- and astrogliosis, Iba1 and GFAP labeling was analyzed in a 200 × 200 µm area around the tachyzoite clusters and of the same region in the brain of the control group was analyzed. The number of voxels representing Iba1 and GFAP labeling with intensities greater than 50 out of 255 (8-bit coding) was quantified and the results were expressed as voxels per µm2 (voxels projected onto an image area). Subsequently, microglia in this area were classified according to activated and non-activated using Imaris 9.9.1 (Oxford Instruments, Abingdon, UK). Surface rendering of all 5 z-stacks was used with the following parameters: surface detail = 0.2 μm, thresholding: absolute intensity 12.7, filter bounding box 250 x 250 nm. All objects consisting of less than 894 voxels (equivalent to a projected area of 1 µm2) were considered ramified, i.e., non-activated, and all objects that were larger were considered amoeboid, i.e., activated. Data were shown as a proportion of the respective microglia population. After data analysis, Adobe Photoshop was used for better visualization using selective gradation curve fitting of the weak DAPI-signal on the nuclei of T. gondii in Figs. 2 and 3 and Supplementary Fig. 1 and for a general gradation curve fitting of all channels in Figs. 4–7 and Supplementary Figs. 1 and 3.
Statistics and reproducibility
A total of 18 guinea pig dams were obtained and randomly divided into a control (n = 9) and infection (n = 9) group. Each fetus was assessed as an individual sample. Numerical source data for all charts are provided as a Supplementary Data file. Statistical analysis was performed using Graphpad Prism 9.4.1 (GraphPad Software Inc., San Diego, USA) software. Normal distribution of all parameters was tested by Anderson-Darling test and Shapiro–Wilk test. T. gondii DNA loads obtained by qPCR analysis and number of apoptotic cells were not normally distributed and analyzed by Mann–Whitney test (for comparison of two groups) and Kruskal–Wallis test (for comparison of more than two groups) followed by Dunn’s post hoc test. All other data were normally distributed and analyzed using one-tailed unpaired t test. P values < 0.05 were considered statistically significant. Significance levels were split further as to **P < 0.01, ***P < 0.001, ****P < 0.0001.
Reporting summary
Further information on research design is available in the Nature Portfolio Reporting Summary linked to this article.
Data availability
Data generated and analyzed during this study are included in this published article or can be obtained from the corresponding author (simone.fietz@vetmed.uni-leipzig.de) on request. Numerical source data for all plots and graphs in the manuscript can be found in Supplementary Data file.
References
Blader, I., Coleman, B., Chen, C.-T. & Gubbels, M.-J. The lytic cycle of Toxoplasma gondii. 15 years later. Annu Rev. Microbiol. 69, 463–485 (2015).
Opsteegh, M., Kortbeek, T. M., Havelaar, A. H. & van der Giessen, J. W. B. Intervention strategies to reduce human Toxoplasma gondii disease burden. Clin. Infect. Dis. 60, 101–107 (2015).
Tenter, A. M., Heckeroth, A. R. & Weiss, L. M. Toxoplasma gondii. From animals to humans. Int. J. Parasitol. 30, 1217–1258 (2000).
Montoya, J. G. & Liesenfeld, O. Toxoplasmosis. Lancet 363, 1965–1976 (2004).
Bigna, J. J. et al. Global, regional, and country seroprevalence of Toxoplasma gondii in pregnant women: a systematic review, modelling and meta-analysis. Sci. Rep. 10, 12102 (2020).
McAuley, J. B. Congenital toxoplasmosis. J. Pediatr. Infect. Dis. Soc. 3(Suppl. 1), S30–S35 (2014).
Dubey, J. P., Lindsay, D. S. & Speer, C. A. Structures of Toxoplasma gondii tachyzoites, bradyzoites, and sporozoites and biology and development of tissue cysts. Clin. Microbiol. Rev. 11, 267–299 (1998).
Dubey, J. P., Miller, N. L. & Frenkel, J. K. The Toxoplasma gondii oocyst from cat feces. J. Exp. Med. 132, 636–662 (1970).
Halonen, S. K. & Weiss, L. M. Toxoplasmosis. Handb. Clin. Neurol. 114, 125–145 (2013).
Ferguson, D. J. & Hutchison, W. M. The host-parasite relationship of Toxoplasma gondii in the brains of chronically infected mice. Virchows Arch. A Pathol. Anat. Histopathol. 411, 39–43 (1987).
Weiss, L. M. & Kim, K. The development and biology of bradyzoites of Toxoplasma gondii. Front. Biosci. 5, D391–D405 (2000).
Schlüter, D. et al. Animals are key to human toxoplasmosis. Int. J. Med. Microbiol. 304, 917–929 (2014).
Chiebao, D. P. et al. Early immune responses and parasite tissue distribution in mice experimentally infected with oocysts of either archetypal or non-archetypal genotypes of Toxoplasma gondii. Parasitology 148, 464–476 (2021).
Cook, A. J. et al. Sources of Toxoplasma infection in pregnant women: European multicentre case-control study. European Research Network on Congenital Toxoplasmosis. BMJ 321, 142–147 (2000).
Meireles, L. R., Ekman, C. C. J., de Andrade, H. F. & Luna, E. J. d. A. Human toxoplasmosis outbreaks and the agent infecting form. Findings from a systematic review. Rev. Inst. Med. Trop. Sao Paulo 57, 369–376 (2015).
Aguirre, A. A. et al. The one health approach to toxoplasmosis: epidemiology, control, and prevention strategies. EcoHealth 16, 378–390 (2019).
Elsheikha, H. M. Congenital toxoplasmosis: priorities for further health promotion action. Public Health 122, 335–353 (2008).
Gilbert, R., Tan, H. K., Cliffe, S., Guy, E. & Stanford, M. Symptomatic Toxoplasma infection due to congenital and postnatally acquired infection. Arch. Dis. Child. 91, 495–498 (2006).
Jones, J. L., Lopez, A., Wilson, M., Schulkin, J. & Gibbs, R. Congenital toxoplasmosis: a review. Obstet. Gynecol. Surv. 56, 296–305 (2001).
Capobiango, J. D. et al. Congenital toxoplasmosis in a reference center of Paraná, Southern Brazil. Braz. J. Infect. Dis. 18, 364–371 (2014).
Fischer, H. G., Nitzgen, B., Reichmann, G., Gross, U. & Hadding, U. Host cells of Toxoplasma gondii encystation in infected primary culture from mouse brain. Parasitol. Res. 83, 637–641 (1997).
Brunet, J. et al. Toxoplasma gondii exploits UHRF1 and induces host cell cycle arrest at G2 to enable its proliferation. Cell. Microbiol. 10, 908–920 (2008).
Parlog, A., Schlüter, D. & Dunay, I. R. Toxoplasma gondii induced neuronal alterations. Parasite Immunol. 37, 159–170 (2015).
Cabral, C. M. et al. Neurons are the primary target cell for the brain-tropic intracellular parasite Toxoplasma gondii. PLoS Pathog. 12, e1005447 (2016).
Kim, M. J. et al. Exosomes secreted by Toxoplasma gondii-infected L6 cells: Their effects on host cell proliferation and cell cycle changes. Korean J. Parasitol. 54, 147–154 (2016).
Wang, G. & Gao, M. Influence of Toxoplasma gondii on in vitro proliferation and apoptosis of hepatoma carcinoma H7402 cell. Asian Pac. J. Trop. Med. 9, 63–66 (2016).
Velásquez, Z. D. et al. Toxoplasma gondii-induced host cellular cell cycle dysregulation is linked to chromosome missegregation and cytokinesis failure in primary endothelial host cells. Sci. Rep. 9, 12496 (2019).
Mouveaux, T. et al. Primary brain cell infection by Toxoplasma gondii reveals the extent and dynamics of parasite differentiation and its impact on neuron biology. Open Biol. 11, 210053 (2021).
Fietz, S. A. & Huttner, W. B. Cortical progenitor expansion, self-renewal and neurogenesis-a polarized perspective. Curr. Opin. Neurobiol. 21, 23–35 (2011).
Dehay, C., Kennedy, H. & Kosik, K. S. The outer subventricular zone and primate-specific cortical complexification. Neuron 85, 683–694 (2015).
Molnár, Z. et al. New insights into the development of the human cerebral cortex. J. Anat. 235, 432–451 (2019).
Villalba, A., Götz, M. & Borrell, V. The regulation of cortical neurogenesis. Curr. Top. Dev. Biol. 142, 1–66 (2021).
Andrews, M. G., Subramanian, L., Salma, J. & Kriegstein, A. R. How mechanisms of stem cell polarity shape the human cerebral cortex. Nat. Rev. Neurosci. 23, 711–724 (2022).
Vaid, S. & Huttner, W. B. Progenitor-based cell biological aspects of neocortex development and evolution. Front. Cell Dev. Biol. 10, 892922 (2022).
Rakic, P. Mode of cell migration to the superficial layers of fetal monkey neocortex. J. Comp. Neurol. 145, 61–83 (1972).
Götz, M., Stoykova, A. & Gruss, P. Pax6 controls radial glia differentiation in the cerebral cortex. Neuron 21, 1031–1044 (1998).
Rakic, P. A small step for the cell, a giant leap for mankind: a hypothesis of neocortical expansion during evolution. Trends Neurosci. 18, 383–388 (1995).
Haubensak, W., Attardo, A., Denk, W. & Huttner, W. B. Neurons arise in the basal neuroepithelium of the early mammalian telencephalon: a major site of neurogenesis. Proc. Natl Acad. Sci. USA 101, 3196–3201 (2004).
Miyata, T. et al. Asymmetric production of surface-dividing and non-surface-dividing cortical progenitor cells. Development 131, 3133–3145 (2004).
Noctor, S. C., Martínez-Cerdeño, V., Ivic, L. & Kriegstein, A. R. Cortical neurons arise in symmetric and asymmetric division zones and migrate through specific phases. Nat. Neurosci. 7, 136–144 (2004).
Hansen, D. V., Lui, J. H., Parker, P. R. L. & Kriegstein, A. R. Neurogenic radial glia in the outer subventricular zone of human neocortex. Nature 464, 554–561 (2010).
Betizeau, M. et al. Precursor diversity and complexity of lineage relationships in the outer subventricular zone of the primate. Neuron 80, 442–457 (2013).
Fietz, S. A. et al. OSVZ progenitors of human and ferret neocortex are epithelial-like and expand by integrin signaling. Nat. Neurosci. 13, 690–699 (2010).
Reillo, I., de Juan Romero, C., García-Cabezas, M. Á. & Borrell, V. A role for intermediate radial glia in the tangential expansion of the mammalian cerebral cortex. Cereb. Cortex 21, 1674–1694 (2011).
Kelava, I. et al. Abundant occurrence of basal radial glia in the subventricular zone of embryonic neocortex of a lissencephalic primate, the common marmoset Callithrix jacchus. Cereb. Cortex 22, 469–481 (2012).
Englund, C. et al. Pax6, Tbr2, and Tbr1 are expressed sequentially by radial glia, intermediate progenitor cells, and postmitotic neurons in developing neocortex. J. Neurosci. 25, 247–251 (2005).
Molyneaux, B. J., Arlotta, P., Menezes, J. R. L. & Macklis, J. D. Neuronal subtype specification in the cerebral cortex. Nat. Rev. Neurosci. 8, 427–437 (2007).
Angevine, J. B. & Sidman, R. L. Autoradiographic study of cell migration during histogenesis of cerebral cortex in the mouse. Nature 192, 766–768 (1961).
Rakic, P. Neurons in rhesus monkey visual cortex: systematic relation between time of origin and eventual disposition. Science 183, 425–427 (1974).
Rakic, P. Specification of cerebral cortical areas. Science 241, 170–176 (1988).
Flori, P. et al. Experimental model of congenital toxoplasmosis in guinea pigs. Use of quantitative and qualitative PCR for the study of maternofetal transmission. J. Med. Microbiol. 51, 871–878 (2002).
Flori, P. et al. Parasite load in guinea pig foetus with real time PCR after maternofoetal transmission of Toxoplasma gondii. Parasite 10, 133–140 (2003).
Grochow, T. et al. Establishment and validation of a guinea pig model for human congenital toxoplasmosis. Parasit. Vectors 14, 389 (2021).
Kasper, L. H., Crabb, J. H. & Pfefferkorn, E. R. Purification of a major membrane protein of Toxoplasma gondii by immunoabsorption with a monoclonal antibody. J. Immunol. 130, 2407–2412 (1983).
Burg, J. L., Perelman, D., Kasper, L. H., Ware, P. L. & Boothroyd, J. C. Molecular analysis of the gene encoding the major surface antigen of Toxoplasma gondii. J. Immunol. 141, 3584–3591 (1988).
Attias, M. et al. The life-cycle of Toxoplasma gondii reviewed using animations. Parasit. Vectors 13, 588 (2020).
Boothroyd, J. C. et al. Genetic and biochemical analysis of development in Toxoplasma gondii. Philos. Trans. R. Soc. Lond. B Biol. Sci. 352, 1347–1354 (1997).
Lendahl, U., Zimmerman, L. B. & McKay, R. D. CNS stem cells express a new class of intermediate filament protein. Cell 60, 585–595 (1990).
Bernhardt, R. & Matus, A. Light and electron microscopic studies of the distribution of microtubule-associated protein 2 in rat brain: a difference between dendritic and axonal cytoskeletons. J. Comp. Neurol. 226, 203–221 (1984).
Shaw, G. & Weber, K. Differential expression of neurofilament triplet proteins in brain development. Nature 298, 277–279 (1982).
Carden, M. J., Trojanowski, J. Q., Schlaepfer, W. W. & Lee, V. M. Two-stage expression of neurofilament polypeptides during rat neurogenesis with early establishment of adult phosphorylation patterns. J. Neurosci. 7, 3489–3504 (1987).
Bignami, A. & Dahl, D. Differentiation of astrocytes in the cerebellar cortex and the pyramidal tracts of the newborn rat. An immunofluorescence study with antibodies to a protein specific to astrocytes. Brain Res. 49, 393–402 (1973).
Kálmán, M. & Hajós, F. Distribution of glial fibrillary acidic protein (GFAP)-immunoreactive astrocytes in the rat brain. I. Forebrain. Exp. Brain Res. 78, 147–163 (1989).
Barami, K., Iversen, K., Furneaux, H. & Goldman, S. A. Hu protein as an early marker of neuronal phenotypic differentiation by subependymal zone cells of the adult songbird forebrain. J. Neurobiol. 28, 82–101 (1995).
Okano, H. J. & Darnell, R. B. A hierarchy of Hu RNA binding proteins in developing and adult neurons. J. Neurosci. 17, 3024–3037 (1997).
Kalusa, M., Heinrich, M. D., Sauerland, C., Morawski, M. & Fietz, S. A. Developmental differences in neocortex neurogenesis and maturation between the altricial dwarf rabbit and precocial guinea pig. Front. Neuroanat. 15, 678385 (2021).
Zhao, Y. O., Khaminets, A., Hunn, J. P. & Howard, J. C. Disruption of the Toxoplasma gondii parasitophorous vacuole by IFNgamma-inducible immunity-related GTPases (IRG proteins) triggers necrotic cell death. PLoS Pathog. 5, e1000288 (2009).
Wang, T. et al. Toxoplasma gondii induce apoptosis of neural stem cells via endoplasmic reticulum stress pathway. Parasitology 141, 988–995 (2014).
Gaggero, G. et al. Neuro-toxoplasmosis and fatal necrotizing cerebellitis. Autops. Case Rep. 12, e2021363 (2022).
Thornberry, N. A. & Lazebnik, Y. Caspases: enemies within. Science 281, 1312–1316 (1998).
Slee, E. A., Adrain, C. & Martin, S. J. Executioner caspase-3, −6, and −7 perform distinct, non-redundant roles during the demolition phase of apoptosis. J. Biol. Chem. 276, 7320–7326 (2001).
Ginhoux, F., Lim, S., Hoeffel, G., Low, D. & Huber, T. Origin and differentiation of microglia. Front. Cell Neurosci. 7, 45 (2013).
Filiano, A. J., Gadani, S. P. & Kipnis, J. Interactions of innate and adaptive immunity in brain development and function. Brain Res. 1617, 18–27 (2015).
Ito, D. et al. Microglia-specific localisation of a novel calcium binding protein, Iba1. Brain Res. Mol. Brain Res. 57, 1–9 (1998).
Okere, C. O. & Kaba, H. Heterogenous immunohistochemical expression of microglia-specific ionized calcium binding adaptor protein (Iba1) in the mouse olfactory bulb. Brain Res. 877, 85–90 (2000).
Leyh, J. et al. Classification of microglial morphological phenotypes using machine learning. Front. Cell Neurosci. 15, 701673 (2021).
Matejuk, A. & Ransohoff, R. M. Crosstalk between astrocytes and microglia: an overview. Front. Immunol. 11, 1416 (2020).
Pusch, L., Romeike, B., Deckert, M. & Mawrin, C. Persistent Toxoplasma bradyzoite cysts in the brain: incidental finding in an immunocompetent patient without evidence of a toxoplasmosis. Clin. Neuropathol. 28, 210–212 (2009).
Wang, T. et al. Toxoplasma gondii: the effects of infection at different stages of pregnancy on the offspring of mice. Exp. Parasitol. 127, 107–112 (2011).
Müller, J. et al. Development of a murine vertical transmission model for Toxoplasma gondii oocyst infection and studies on the efficacy of bumped kinase inhibitor (BKI)-1294 and the naphthoquinone buparvaquone against congenital toxoplasmosis. J. Antimicrob. Chemother. 72, 2334–2341 (2017).
Dard, C. et al. Management of toxoplasmosis in transplant recipients: an update. Expert Rev. Anti Infect. Ther. 16, 447–460 (2018).
Samojłowicz, D. et al. Presence of Toxoplasma gondii infection in brain as a potential cause of risky behavior: a report of 102 autopsy cases. Eur. J. Clin. Microbiol. Infect. Dis. 38, 305–317 (2019).
Vyas, A., Kim, S.-K., Giacomini, N., Boothroyd, J. C. & Sapolsky, R. M. Behavioral changes induced by Toxoplasma infection of rodents are highly specific to aversion of cat odors. Proc. Natl Acad. Sci. USA 104, 6442–6447 (2007).
Di Cristina, M. et al. Temporal and spatial distribution of Toxoplasma gondii differentiation into bradyzoites and tissue cyst formation in vivo. Infect. Immun. 76, 3491–3501 (2008).
Berenreiterová, M., Flegr, J., Kuběna, A. A. & Němec, P. The distribution of Toxoplasma gondii cysts in the brain of a mouse with latent toxoplasmosis: implications for the behavioral manipulation hypothesis. PLoS ONE 6, e28925 (2011).
Figueiredo, C. A. et al. Immune response and pathogen invasion at the choroid plexus in the onset of cerebral toxoplasmosis. J. Neuroinflammation 19, 17 (2022).
Ross, E. C., Olivera, G. C. & Barragan, A. Early passage of Toxoplasma gondii across the blood-brain barrier. Trends Parasitol. 38, 450–461 (2022).
Melzer, T. C., Cranston, H. J., Weiss, L. M. & Halonen, S. K. Host cell preference of Toxoplasma gondii cysts in murine brain: a confocal study. J. Neuroparasitol. 1, N100505 (2010).
Mendez, O. A. & Koshy, A. A. Toxoplasma gondii: Entry, association, and physiological influence on the central nervous system. PLoS Pathog. 13, e1006351 (2017).
Marcos, A. C. et al. Toxoplasma gondii infection impairs radial glia differentiation and its potential to modulate brain microvascular endothelial cell function in the cerebral cortex. Microvasc. Res. 131, 104024 (2020).
Pires, L. B. et al. Infection of mouse neural progenitor cells by Toxoplasma gondiireduces proliferation, migration, and neuronal differentiation in vitro. Am. J. Pathol. 193, 977–994 (2023).
Wong, F. K. et al. Sustained Pax6 expression generates primate-like basal radial glia in developing mouse neocortex. PLoS Biol. 13, e1002217 (2015).
Stepien, B. K., Vaid, S. & Huttner, W. B. Length of the neurogenic period-a key determinant for the generation of upper-layer neurons during neocortex development and evolution. Front. Cell Dev. Biol. 9, 676911 (2021).
Molestina, R. E., El-Guendy, N. & Sinai, A. P. Infection with Toxoplasma gondii results in dysregulation of the host cell cycle. Cell. Microbiol 10, 1153–1165 (2008).
Koshy, A. A. et al. Toxoplasma co-opts host cells it does not invade. PLoS Pathog. 8, e1002825 (2012).
Chang, S. et al. Toxoplasma gondii rhoptry protein ROP16 mediates partially SH-SY5Y cells apoptosis and cell cycle arrest by directing Ser15/37 phosphorylation of p53. Int. J. Biol. Sci. 11, 1215–1225 (2015).
Lee, J. C., Mayer-Proschel, M. & Rao, M. S. Gliogenesis in the central nervous system. Glia 30, 105–121 (2000).
Rowitch, D. H. & Kriegstein, A. R. Developmental genetics of vertebrate glial-cell specification. Nature 468, 214–222 (2010).
Robel, S., Berninger, B. & Götz, M. The stem cell potential of glia: lessons from reactive gliosis. Nat. Rev. Neurosci. 12, 88–104 (2011).
Lange Canhos, L. et al. Repetitive injury and absence of monocytes promote astrocyte self-renewal and neurological recovery. Glia 69, 165–181 (2021).
Cowan, M. N., Sethi, I. & Harris, T. H. Microglia in CNS infections: insights from Toxoplasma gondii and other pathogens. Trends Parasitol. 38, 217–229 (2022).
Verney, C., Monier, A., Fallet-Bianco, C. & Gressens, P. Early microglial colonization of the human forebrain and possible involvement in periventricular white-matter injury of preterm infants. J. Anat. 217, 436–448 (2010).
Schlegelmilch, T., Henke, K. & Peri, F. Microglia in the developing brain: from immunity to behaviour. Curr. Opin. Neurobiol. 21, 5–10 (2011).
Swinnen, N. et al. Complex invasion pattern of the cerebral cortex bymicroglial cells during development of the mouse embryo. Glia 61, 150–163 (2013).
Tay, T. L., Savage, J. C., Hui, C. W., Bisht, K. & Tremblay, M.-È. Microglia across the lifespan: from origin to function in brain development, plasticity and cognition. J. Physiol. 595, 1929–1945 (2017).
Hattori, Y. The behavior and functions of embryonic microglia. Anat. Sci. Int. 97, 1–14 (2022).
Brahmachari, S., Fung, Y. K. & Pahan, K. Induction of glial fibrillary acidic protein expression in astrocytes by nitric oxide. J. Neurosci. 26, 4930–4939 (2006).
Dellacasa-Lindberg, I. et al. Migratory activation of primary cortical microglia upon infection with Toxoplasma gondii. Infect. Immun. 79, 3046–3052 (2011).
Burrells, A. et al. Detection and dissemination of Toxoplasma gondii in experimentally infected calves, a single test does not tell the whole story. Parasit. Vectors. 11, 45 (2018).
Belaz, S., Gangneux, J.-P., Dupretz, P., Guiguen, C. & Robert-Gangneux, F. A ten-year retrospective comparison of two target sequences, REP-529 and B1, for Toxoplasma gondii detection by quantitative PCR. J. Clin. Microbiol. 53, 1294–1300 (2015).
Bier, N. S. et al. Performance of three molecular methods for detection of Toxoplasma gondii in pork. Food Waterborne Parasitol. 14, e00038 (2019).
Talabani, H. et al. Contributions of immunoblotting, real-time PCR, and the Goldmann-Witmer coefficient to diagnosis of atypical toxoplasmic retinochoroiditis. J. Clin. Microbiol. 47, 2131–2135 (2009).
Hoffmann, B., Depner, K., Schirrmeier, H. & Beer, M. A universal heterologous internal control system for duplex real-time RT-PCR assays used in a detection system for pestiviruses. J. Virol. Methods 136, 200–209 (2006).
Schares, G. et al. Sensitive, quantitative detection of Besnoitia darlingi and related parasites in intermediate hosts and to assess felids as definitive hosts for known and as-yet undescribed related parasite species. Int. J. Parasitol. Parasites Wildl. 11, 114–119 (2020).
Sauerland, C. et al. The basal radial glia occurs in marsupials and underlies the evolution of an expanded neocortex in therian mammals. Cereb. Cortex 28, 145–157 (2018).
Acknowledgements
We thank Yasmina Schmitt, Josephine Schiffner, Andrea Bärwald, Alrik-Markis Kunisch, Mareen Tuschy, Susanne Zahnow, Jenny Mein, and Gregor Pfeiffer for their technical support as well as Katharina Rauhe and Katrin Balzejak for their support in oocyst collection. Moreover, we thank Hans-Jürgen Raqué for providing the ultrasonography equipment and Johannes Kauffold and Haukur Sigmarsson for their help in obtaining medications. We thank Dr. Jan Schinköthe (Institute of Veterinary Pathology, Faculty of Veterinary Medicine, Leipzig University) for providing the brain image used in Fig. 2c. We are thankful for the technical and conceptual support provided by the BioImaging Core Facility, Leipzig University. We acknowledge the support provided by the National Research Platform for Zoonoses/Federal Ministry of Education and Research (01KI1801), and the Research Academy Leipzig and the Vice-Rector for Research and Young Academics (Pre-Doc-Award conferred to T.G. and S.A.F.), University of Leipzig, Germany.
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S.A.F. conceived the study. S.A.F. and A.D. designed and supervised the study. T.G. performed infection of animals, euthanasia, dissection, tissue homogenization, DNA extraction, qPCR, immunohistochemistry, microscopy and data analysis. B.B. performed cycle synchronization and assisted in dissection of animals. G.S. and P.M. established qPCR protocol and performed serological investigation. J.K. established cell quantification protocol. L.R. performed ultrasonographic pregnancy examination. C.S. contributed oocysts. T.G., Z.R.-S., G.S., P.M., J.K., A.D., and S.A.F. discussed data. T.G. and S.A.F. wrote the paper. A.D., Z.R.S., C.S., and J.K. edited the paper. All authors read and approved the manuscript.
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Grochow, T., Beck, B., Rentería-Solís, Z. et al. Reduced neural progenitor cell count and cortical neurogenesis in guinea pigs congenitally infected with Toxoplasma gondii. Commun Biol 6, 1209 (2023). https://doi.org/10.1038/s42003-023-05576-6
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DOI: https://doi.org/10.1038/s42003-023-05576-6
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