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Original Research ARTICLE

Front. Neuroanat., 27 February 2018 | https://doi.org/10.3389/fnana.2018.00013

Neural Damage in Experimental Trypanosoma brucei gambiense Infection: Hypothalamic Peptidergic Sleep and Wake-Regulatory Neurons

  • 1Department of Neuroscience Biomedicine and Movement Sciences, University of Verona, Verona, Italy
  • 2Institut National de Recherche Biomédicale (INRB), Kinshasa, Democratic Republic of Congo
  • 3National Institute of Neuroscience (INN), Verona Unit, Verona, Italy

Neuron populations of the lateral hypothalamus which synthesize the orexin (OX)/hypocretin or melanin-concentrating hormone (MCH) peptides play crucial, reciprocal roles in regulating wake stability and sleep. The disease human African trypanosomiasis (HAT), also called sleeping sickness, caused by extracellular Trypanosoma brucei (T. b.) parasites, leads to characteristic sleep-wake cycle disruption and narcoleptic-like alterations of the sleep structure. Previous studies have revealed damage of OX and MCH neurons during systemic infection of laboratory rodents with the non-human pathogenic T. b. brucei subspecies. No information is available, however, on these peptidergic neurons after systemic infection with T. b. gambiense, the etiological agent of 97% of HAT cases. The present study was aimed at the investigation of immunohistochemically characterized OX and MCH neurons after T. b. gambiense or T. b. brucei infection of a susceptible rodent, the multimammate mouse, Mastomys natalensis. Cell counts and evaluation of OX fiber density were performed at 4 and 8 weeks post-infection, when parasites had entered the brain parenchyma from the periphery. A significant decrease of OX neurons (about 44% reduction) and MCH neurons (about 54% reduction) was found in the lateral hypothalamus and perifornical area at 8 weeks in T. b. gambiense-infected M. natalensis. A moderate decrease (21% and 24% reduction, respectively), which did not reach statistical significance, was found after T. b. brucei infection. In two key targets of diencephalic orexinergic innervation, the peri-suprachiasmatic nucleus (SCN) region and the thalamic paraventricular nucleus (PVT), densitometric analyses showed a significant progressive decrease in the density of orexinergic fibers in both infection paradigms, and especially during T. b. gambiense infection. Altogether the findings provide novel information showing that OX and MCH neurons are highly vulnerable to chronic neuroinflammatory signaling caused by the infection of human-pathogenic African trypanosomes.

Introduction

Many infections disturb sleep, and somnolence is part of the so-called sickness behavior in response to infections (Poon et al., 2015). The alterations of sleep in human African trypanosomiasis (HAT) are, however, so characteristic and severe that they gave to the disease the alternative name of sleeping sickness (Buguet et al., 2014; Büscher et al., 2017). HAT is caused by the extracellular protozoan parasites Trypanosoma brucei (T. b.), inoculated through bites of the hematophagous tsetse flies (genus Glossina). The disease is still endemic, with a focal distribution mostly in remote rural areas, in the vast sub-Saharan region of the vector’s habitat. After an epidemic in the 1990s, this neglected tropical disease has attracted attention in the public health agenda. Due to sustained control activities, the reported cases have declined in recent years (dropping to less than 3000 in 2015) and the disease is currently targeted for elimination (WHO, 2017). There are, however, concerns on the fight against HAT and worries about disease re-emergence, especially due to inaccurate case reporting and to silent carriers (Welburn et al., 2016; Büscher et al., 2017).

The vast majority of HAT cases (97%; WHO, 2017) are due to the infection of T. b. gambiense, for which humans provide the reservoir, causing a chronic progressive form of the disease with a course from 1 to 3 years. T. b. gambiense HAT is endemic in western and central Africa, and especially in the Democratic Republic of Congo (DRC) where over 70% of cases in the last 10 years have been reported (WHO, 2017). A more acute form of HAT, lasting 6–8 months, is endemic in eastern and southern Africa and is caused by T. b. rhodesiense, representing a zoonosis with wildlife and livestock reservoirs and therefore difficult to control. Most experimental studies on nervous system infection caused by African trypanosomes have been performed using a third parasite subspecies, T. b. brucei, which is infectious to animals but not to humans.

During the progression of T. b. infection, the parasites, which initially invade peripheral organs through the blood and lymph, enter the central nervous system parenchyma. HAT is considered fatal if untreated (WHO, 2017) and the therapy of the meningoencephalitic stage is very toxic. Ongoing clinical trials based on oral therapy with fexinidazole are opening new perspectives for the cure of HAT (Mesu et al., 2018).

The disease causes severe chronic neuroinflammation, with high levels of inflammatory mediators (Kennedy, 2013; Büscher et al., 2017). Early autoptic studies of HAT victims have shown glial activation with myelin pallor but no features of neurodegeneration (Lejon et al., 2013). The clinical picture, initially nonspecific, leads to a constellation of neurological and psychiatric alterations during disease progression (Kennedy, 2013; Lejon et al., 2013; Buguet et al., 2014; Büscher et al., 2017). Since historical descriptions, striking clinical features of HAT in endemic regions are represented by diurnal somnolence and nocturnal insomnia, as well as episodes of irresistible sleep during wakefulness (sleep attacks; Lhermitte, 1910; Blum et al., 2006; Buguet et al., 2014). Polysomnographic recordings of the sleep-wake cycle in HAT patients have shown that the disease does not cause hypersomnia but rather a circadian disruption of sleep-wake alternation, as well as alterations of the sleep structure (Buguet et al., 2001, 2005, 2014).

Sleep-wake cycle changes during African trypanosomiasis implicate the master circadian pacemaker, the hypothalamic suprachiasmatic nucleus (SCN), which drives endogenous biological rhythms in the mammalian brain (van Esseveldt et al., 2000; Golombek and Rosenstein, 2010; Moore, 2013). Findings on neuronal cell loss in the SCN of an animal model of T. b. gambiense infection provided by the multimammate mouse, Mastomys natalensis (Mehlitz, 1975; Büscher et al., 2005) are presented in a companion article (Tesoriero et al., 2018). On the other hand, alterations of sleep architecture in African trypanosomiasis implicate damage to structures of the distributed neural network which regulates sleep and wakefulness (Saper et al., 2010; Scammell et al., 2017). In particular, the observation of sudden sleep episodes during wakefulness, as well as sleep fragmentation and disruption of the normal sleep sequence which also occur in T. b. brucei-infected rats (Darsaud et al., 2003; Seke Etet et al., 2012; Laperchia et al., 2016, 2017) recall the chronic sleep disorder narcolepsy (Sateia, 2014; Scammell, 2015), whose pathogenesis is due to impaired orexinergic signaling (Liblau et al., 2015). Such alterations point, therefore, to dysfunction of neurons which contain the orexin (OX)/hypocretin peptides, located in the posterior lateral hypothalamus. These neurons play a key role in wakefulness stability and sleep-wake transitions (de Lecea and Huerta, 2014), besides their implication in energy homeostasis and other physiological functions underlying motivated behaviors (Sakurai, 2014; Li et al., 2016).

Orexinergic neurons are intermingled with those expressing another peptide, melanin-concentrating hormone (MCH), which are sleep-promoting and also regulate food intake and other functions implicated in the motivational aspects of behavior (Torterolo et al., 2015; Ferreira et al., 2017). Structural and functional alterations of these two major hypothalamic neuronal populations has been previously reported in T. b. brucei-infected laboratory rats and mice (Palomba et al., 2015), but no information on these cell groups during T. b. gambiense infection is available. To fill this gap of knowledge, the present study was aimed at the histopathological investigation of OX and MCH cell bodies and OX fibers in the animal model of T. b. gambiense infection provided by M. natalensis. This rodent is sensitive to T. b. gambiense infection (Mehlitz, 1978), at variance with laboratory rodents which are not susceptible to most isolates of this human-pathogenic parasite subspecies (Giroud et al., 2009).

OX neurons give origin to extensive projections (Peyron et al., 1998). In particular, in laboratory rodents orexinergic fibers innervate the area surrounding the SCN (Peyron et al., 1998; Marston et al., 2008), and show a discrete distribution in the thalamus along the midline with dense innervation of the thalamic paraventricular nucleus (PVT; Peyron et al., 1998; McGranaghan and Piggins, 2001; Mintz et al., 2001; Kirouac et al., 2005) documented also in African rodents (Bhagwandin et al., 2011a). The density of OX innervation was here evaluated in these two diencephalic targets of orexinergic projections, the peri-SCN region and PVT, given their high functional relevance for interactions between circadian and vigilance state regulation (Colavito et al., 2015).

Materials and Methods

Animals and Infection

Experimental procedures were performed under approval of the ethical committee of the Ministry of Health of DRC, adhering to the European Communities Council (86/609/EEC) directives and the ARRIVE (“Animal Research Reporting of in vivo Experiments”) guidelines. All efforts were made to minimize animal number and suffering. The present investigation was based on the same brains of the animals used for the study of the SCN presented in a companion article (Tesoriero et al., 2018).

In brief, adult M. natalensis of both sexes (a total number of 45 animals, 30 destined to the two infection paradigms and 15 controls) were obtained from the breeding colony at the Institut National de Recherche Biomedicale (INRB, Kinshasa, DRC).

The rodent M. natalensis is very widespread in sub-Saharan Africa, and holds a taxonomic position between the mouse (house mouse) and the rat (ship, roof rat; Coetzee, 1975). The definition of multimammate derives from a uniquely large number of mammae in the female (Isaäcson, 1975). M. natalensis (also called Praomys natalensis) is nocturnal, with the peak of activity in the first 3 h of the period of darkness (Coetzee, 1975). The animal is omnivorous, uses preferentially burrows of other rodents for nesting and adapts easily to different environments (Isaäcson, 1975), representing the major rodent pest in sub-Saharan Africa (e.g., Mulungu et al., 2013).

The animals were maintained under a 12 h:12 h light/dark cycle, with free access to food and water. One group of animals was infected with T. b. gambiense (MHOM/INRB/2006/11A, originally isolated from a patient in DRC in 2006), and another group with T. b. brucei (AnTat 1.1E). The parasites derived from the cryostabilates collected at INRB, and each experimental group of infected M. natalensis included matched uninfected controls. The infection was done with intraperitoneal injection of 0.25 ml per animal of a solution (0.1 M phosphate buffer, pH 7.4, supplemented with glucose) containing 106.9–107.2 trypanosomes/ml. Parasitaemia was verified weekly from the tip of the tail vein. At 4 and 8 weeks post-infection, the animals (n = 3 or 4 infected animals per time point and control animals per experimental group) were sacrificed during daytime, under anesthesia, by transcardial perfusion with ice-cold 0.9% saline followed by formaldehyde solution (obtained dissolving paraformaldehyde in 0.1 M phosphate buffer, pH 7.2, at a 4% concentration). Previous monitoring at INRB of the natural course of the infections in M. natalensis indicated that at 8 weeks T. b. brucei infection is in a very advanced phase (and this was therefore selected as end-point of the study), whereas T. b. gambiense infection can last several weeks.

After perfusion, the brains were removed from the skull, posfixed for a few hours, and then stored until processing at 4°C in 0.01 M phosphate buffered-saline, pH 7.4 (PBS), containing 0.1% sodium azide.

Tissue Processing and Immunohistochemistry

Following cryoprotection in 30% sucrose in PBS, the brains were cut on the coronal plane with a freezing microtome into 30 μm-thick sections, which were collected in six series. One series of sections was stained with cresyl violet for cytoarchitectonic control.

Two series of sections through the hypothalamus were processed free-floating for OX immunohistochemistry. The peptides OX-A and OX-B, also called hypocretin-1 and 2, cleaved from the common precursor prepro-OX, are largely co-localized in the same neurons (Nixon and Smale, 2007), and OX-A is more stable than OX-B. OX-A immunophenotyping was therefore used to investigate orexinergic neurons in the present study. The sections were first soaked in 1% H2O2 in PBS for 20 min to inactivate endogenous peroxidase activity, and then pre-incubated in a solution of 5% bovine serum albumin (BSA) and 0.3% Triton X-100 in PBS for 1 h at room temperature. Subsequently, the sections were incubated overnight at room temperature in polyclonal goat anti-OX-A antibody (1:500; Santa Cruz, CA, USA) diluted in PBS containing 1% BSA, 0.2% Triton X-100. Following thorough washes, the sections were incubated for 2 h in biotinylated horse anti-goat IgGs (1:200, Vector, Burlingame, CA, USA), and finally reacted with avidin-peroxidase complex (1:100, Vector, Burlingame, CA, USA) for 1 h and with 3,3′-diaminobenzidine (DAB) as chromogen.

The second series was processed further for MCH immunohistochemistry based on a two-color protocol (Peng et al., 1995). These sections were incubated overnight at room temperature in polyclonal rabbit anti-MCH antibody (1:1000; Phoenix Pharmaceuticals, Burlingame, CA, USA). After repeated washing, the sections were incubated for 2 h in biotinylated goat anti-rabbit IgGs (1:200, Vector) and then reacted with avidin-peroxidase complex (1:100; Vector) for 1 h. In the last step of the procedure, the sections were reacted in a freshly prepared and filtered solution containing 0.05% α-naphthol, 0.1% ammonium carbonate, and 0.003% H2O2 in PBS. The dark blue reaction product was turned into pink by an additional incubation in 0.1% phosphate-buffered pyronin B. This procedure results in the simultaneous visualization in bright-field microscopy of brown DAB reaction products of the first incubation and pink reaction products of the second run (Peng et al., 1995).

After immunohistochemical processing, all sections were thoroughly washed in PBS, mounted on gelatin-coated slides, air-dried, dehydrated, cleared and coverslipped with Entellan. Specific immunostaining was absent in control sections in which the primary antibodies were omitted.

The presence of parasites in the brain parenchyma was investigated in additional sections through the telencephalon and diencephalon, which were processed for double immunofluorescence. These sections were incubated with a mixture of primary antibodies: rabbit polyclonal antibodies which recognize the anti-variant surface glycoprotein of the AnTat 1:1E stabilate (1:200; kindly provided by Philippe Büscher, Institute of Tropical Medicine, Antwerp, Belgium) to visualize the parasites, and goat polyclonal anti-glucose transporter-1 antibodies (1:100, Santa Cruz Biotechnology) to visualize blood vessel endothelia (Pardridge et al., 1990). The sections were rinsed in PBS and incubated in a solution of species-specific secondary antibodies conjugated with Cy2 or Cy3 (1:100; Jackson ImmunoResearch, Suffolk, UK), rinsed in PBS, mounted on slides using a fluorescence-compatible medium (Dako, Hamburg, Germany) and stored at 4°C.

Data Analysis and Statistics

The sections processed for immunofluorescence for parasite detection were observed with a confocal laser scanning microscope (Zeiss LSM 510 Carl Zeiss, Jena, Germany), equipped with an argon laser emitting at 488 nm (Cy2) and a helium/neon laser emitting at 543 nm (Cy3). The other sections were investigated in bright-field microscopy and quantitative analyses were pursued in three animals per group, blindly of the animal’s experimental group assignment.

The series of sections processed for OX-A single immunohistochemistry was used for OX cell counts, and that processed for double immunohistochemistry for MCH cell counts. The number of OX and MCH cells was determined stereologically using the optical fractionator method throughout the rostrocaudal extent of the perifornical area and lateral hypothalamus. Cells were visualized using an Olympus BX51 microscope (20× objective) with a motorized stage connected to a digital camera (JVC CCD KY-F58) and equipped with the image analysis digital system Stereo-Investigator software (MicroBrightfield Corp.). For a systematic random sampling, a grid centered on the fornix and adjacent medially to the wall of the third ventricle was used. The grid was divided into nine counting frames, allowing also partial cell counts in the medial, middle and lateral portions of the lateral hypothalamus. Only cells within the frame or touching one of the frame borders were counted.

For densitometric evaluation, three regularly spaced sections were sampled through the middle portion of the SCN and PVT, respectively, from each animal. In each section, under calibrated constant light parameters, four images from the PVT and two images from the peri-SCN region (within an area of 300 μm in length lateral to the SCN) were randomly sampled on each side using a 40× objective (NA 0.75; yielding a frame of 0.0256 mm2). OX immunoreactivity signal was then measured by defining the zero value of optical density (OD) as background, measured in a portion of the section tissue devoid of specific immunostaining. For each region of interest (ROI), the values from each section were averaged. A grand mean for each ROI was then computed from the mean value derived from each section.

Data are reported as mean ± standard error of the mean (SEM). Kruskal-Wallis analysis of variance followed by the Dunn’s test for pairwise comparison was used for the statistical evaluation of cell counts. One-way analysis of variance followed by the LSD post hoc test was used for OD values of immunoreactivity of OX fibers in the peri-SCN region and PVT. Significance threshold was set at P < 0.05.

Results

Trypanosomes in the Brain Parenchyma

Double immunofluorescence showed in M. natalensis the occurrence of T. b. gambiense and T. b. brucei outside blood vessels within the brain parenchyma, in variable amounts, at both 4 weeks and 8 weeks (Figure 1) after infection, as also presented in the companion article (Tesoriero et al., 2018). This indicated that in both paradigms the infection was in the encephalitic stage at the sampled time points.

FIGURE 1
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Figure 1. Confocal microscopy images showing parasites (in red) in the brain parenchyma at 8 weeks (W) after Trypanosoma brucei brucei (Tbb) or Trypanosoma brucei gambiense (Tbg) systemic infection. Blood vessel walls are visualized by anti-glucose transporter-1 immunolabeling (in green). Scale bar: 40 μm.

OX and MCH Cell Bodies

In M. natalensis, OX-immunolabeled neurons showed a distribution similar to that described in laboratory rodents (Peyron et al., 1998; Mintz et al., 2001) and in a variety of African rodents (Bhagwandin et al., 2011a,b; Sweigers et al., 2017). The largest population was concentrated in the perifornical area, from which it extended to the lateral hypothalamus (Figure 2). MCH neurons also showed in the hypothalamus the distribution described in rodents, very similar, in particular, to that reported in the rat (Bittencourt, 2011). Thus, MCH neurons were distributed rostrally in the incerto-hypothalamic area, between the fornix and the internal capsule at the level of the tuberal lateral hypothalamus. Proceeding posteriorly, MCH neurons were densely aggregated around the fornix, and with sparser distribution medially to the internal capsule, as well as dorsally in the zona incerta, and with a medial, periventricular location. MCH neurons were intermingled with OX neurons in the perifornical area and lateral hypothalamus, and also surrounded OX neurons dorsally and ventrally. OX and MCH somata were morphologically similar, with a multipolar or fusiform shape (Figures 3A,B, 4), giving origin to varicose fibers.

FIGURE 2
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Figure 2. Low power view of orexin (OX)-A-immunoreactive neurons in the perifornical area and lateral hypothalamus of Mastomys natalensis at 4 weeks (W) and 8 W after infection with Trypanosoma brucei brucei (Tbb) or Trypanosoma brucei gambiense (Tbg) and in uninfected animals. Note the rarefaction of immunostained cell bodies and the reduction of neuropil immunolabeling in the infected animals. Abbreviations: f, fornix; opt, optic tract. Scale bar: 250 μm.

FIGURE 3
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Figure 3. (A,B) Images of orexin-A-immunoreactive neurons in uninfected Mastomys natalensis (B represents at higher power the area boxed in A), and at 4 weeks (W) and 8 W after infection with Trypanosoma brucei brucei (Tbb) or Trypanosoma brucei gambiense (Tbg) (C–F). Abbreviations: f, fornix; opt, optic tract. Scale bars: 250 μm in (A), 150 μm in (E) (applies also to B–D,F).

FIGURE 4
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Figure 4. Images of OX-A-immunoreactive neurons (brown) and melanin-concentrating hormone (MCH)-immunoreactive neurons (purple) through the middle third (upper row) and posterior third (lower row) of the lateral hypothalamus of uninfected Mastomys natalensis and at 8 weeks (W) after infection with Trypanosoma brucei brucei (Tbb) or Trypanosoma brucei gambiense (Tbg). Note the marked shrinkage of many MCH-immunostained neurons. Scale bar: 150 μm.

A decrease in the density of OX cell bodies and neuropil immunostaining after African trypanosome infection at both the sampled time points was evident even at low power observation along the rostrocaudal and mediolateral axes (Figure 2). At higher power, the intensity of the soma immunostaining appeared relatively preserved in the infected animals, but with less extensive dendritic filling than in matched controls, and some cell bodies appeared shrunken (Figures 3C–F). Also the density of MCH neurons appeared decreased in both paradigms of infection, with shrinkage of many cell bodies (Figure 4).

Cell counts documented a progressive decrease of both peptidergic cell populations, which was more marked after T. b. gambiense infection than in the T. b. brucei-infected animals (Figure 5). In particular, after T. b. brucei infection the reduction of OX-immunostained cells with respect to controls was 11.12 ± 6.8% at 4 weeks and 21.34 ± 9.8% at 8 weeks, and that of the MCH-immunostained cells, evaluated in the lateral hypothalamus and perifornical area, was 17.53 ± 10.6% at 4 weeks and 24.45 ± 2.2% at 8 weeks. These decreases did not reach, however, statistical significance. After T. b. gambiense infection, 21.58 ± 7.6% reduction of OX-immunostained cells was documented at 4 weeks, and 43.78 ± 7.4% reduction at 8 weeks, when the cell number decrease vs. matched controls was significant. Even more marked was the decrease of MCH neurons (48.15 ± 4% reduction at 4 weeks and 54.15 ± 6.3% at 8 weeks), which was significant at both survival times.

FIGURE 5
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Figure 5. The bar graphs illustrate the stereological counts of neurons containing OX-A (A,B) or MCH (C,D) in control (ctrl) Mastomys natalensis and at 4 weeks (W) and 8 W after infection with Trypanosoma brucei (T. b.) brucei (A,C) or T. b. gambiense (B,D). *P < 0.05; **P < 0.001.

Partial cell counts showed that loss of immunostained cell bodies occurred throughout the extent of their distribution in the lateral hypothalamus and perifornical area.

OX Fibers

In uninfected M. natalensis, orexinergic fibers were found to be densely aggregated laterally to the SCN, as well as along the thalamic midline, innervating PVT throughout its extent. A significant density decrease was found in the orexinergic innervation of the peri-SCN region at 4 and 8 weeks after T. b. brucei infection (Figure 6). In PVT, T. b. brucei infection resulted in a reduction of orexinergic fiber density at 4 weeks, which was further reduced, and significant, at 8 weeks (Figure 7). In the peri-SCN region of T. b. gambiense-infected animals the decrease in the density of orexinergic fibers was very marked and highly significant at 8 weeks (Figure 6). Extreme reduction of orexinergic innervation was found in PVT at both 4 and 8 weeks after T. b. gambiense infection (Figures 7, 8).

FIGURE 6
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Figure 6. Top: images of the ventral part of the anterior hypothalamus showing OX-A immunoreactive fibers in the region lateral to the suprachiasmatic nucleus (SCN, delimited by adotted line), in Mastomys natalensis at 4 weeks (W) and 8 W after infection with Trypanosoma brucei brucei (Tbb) or Trypanosoma brucei gambiense (Tbg). Note that the decrease in the immunoreactive fiber density, especially at 8 weeks after T. b. gambiense infection. Scale bar: 250 μm. Bottom: bar graphs of the quantitative densitometric evaluation of OX-A immunosignal in the peri-SCN region in control (ctrl) and infected animals. *P < 0.05; ***P < 0.001. Abbreviations:OD, optical density; OX, optic chiasm.

FIGURE 7
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Figure 7. Top: images of the paraventricular thalamic nucleus (PVT) of Mastomys natalensis showing OX-A-immunoreactive fibers at 4 weeks (W) and 8 W after infection with Trypanosoma brucei brucei (Tbb) or Trypanosoma brucei gambiense (Tbg). Note the marked decrease of PVT orexinergic innervation, especially after T. b. gambiense infection (see also Figure 6). Scale bar: 250 μm. Bottom: bar graphs of the quantitative densitometric evaluation (OD, optical density) of OX-A immunosignal in PVT of control (ctrl) and infected animals. *P < 0.05; ***P < 0.001.

FIGURE 8
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Figure 8. Images of orexin-A-immunoreactive preterminal and fibers in the paraventricular thalamic nucleus of uninfected Mastomys natalensis (A,C) and at 8 weeks after infection with Trypanosoma brucei gambiense (B,D). (C,D) represent at higher magnification fields of (A,B), respectively, as indicated by the asterisks for spatial landmark. Note in (C) the abundance of varicose fibers in the control animals and note in (D) their marked decrease and fragmentation in the infected animal. Abbreviation: D3V, dorsal third ventricle. Abbreviation: D3V, dorsal third ventricle. Scale bars: 200 μm in (A,B), 50 μm in (C,D).

Discussion

The present findings show that T. b. gambiense infection leads to progressive quantitative decrease of OX and MCH neurons, and that this is more marked than that caused by T. b. brucei infection in the same host species, susceptible to both parasite subspecies. At the endpoint of the study (8 weeks post-infection), the reduction of OX neurons in M. natalensis was about 44% and that of MCH neurons accounted for the loss of about 54% of these neurons in the lateral hypothalamus and perifornical area. Of note, considerable damage of MCH neurons was documented in M. natalensis also at an earlier phase of the encephalitis (about 48% reduction of MCH neurons and about 21% reduction of OX neurons at 4 weeks post-infection).

Immunophenotyping could not here reveal whether the decrease was due to cell death phenomena or downregulation of peptide expression below the threshold of immunohistochemical visualization. However, in the infected animals immunostaining showed cell damage suggestive of an ongoing degenerative process, previously documented also in T. b. brucei-infected laboratory rodents in the absence of overall cell loss in the hypothalamus (Palomba et al., 2015).

The present analyses in infected M. natalensis also demonstrated significantly impoverished orexinergic innervation, which was especially marked after T. b. gambiense infection. This was here shown in the peri-SCN region, which is in turn involved in the circadian control of OX neuron activation (Marston et al., 2008; Belle et al., 2014; Belle and Piggins, 2017) that could be thus impaired during the infection. Decreased orexinergic input was also here documented in PVT, the thalamic midline structure in which OX release exerts powerful functional effects, and which plays a key role in funnelling state-dependent behavior information into the limbic system and prefrontal cortex (Colavito et al., 2015).

Loss of OX neurons (90% or greater) is the neuropathological hallmark of narcolepsy, and in particular of narcolepsy with cataplexy (sudden loss of postural muscle tone, triggered especially by emotion; Peyron et al., 2000; Thannickal et al., 2000). OX neurons degenerate also in narcolepsy without cataplexy, as reported in a post-mortem brain examination which showed loss of 33% of OX neurons (Thannickal et al., 2009). Besides narcoleptic-like changes of sleep architecture in HAT, the clinical phenotype of the sleep-wake cycle is, however, very different in this disease and in narcolepsy, since narcolepsy does not include circadian rhythm disturbances (Dantz et al., 1994).

The investigation of OX levels in the cerebrospinal fluid (CSF) of T. b. gambiense HAT patients (Dauvilliers et al., 2008) and T. b. brucei-infected rats (Palomba et al., 2015) have shown a decrease, which, however, was not significant and exhibited high interindividual variability. The concentration of OX in the CSF of narcoleptics with typical cataplexy is very low, whereas it is normal in most cases of narcolepsy without cataplexy, as well as in other neurodegenerative or neurotraumatic conditions which lead to partial loss of OX neurons (Bourgin et al., 2008). On the other hand, experimental evidence based on lesions of OX neurons in the rat has shown that a very large cell loss is needed to impair OX level in the CSF, which points to a considerable compensatory capacity of surviving OX neurons (Gerashchenko et al., 2003).

Importantly, polysomnographic recording of a limited cohort of T. b. gambiense HAT patients has shown that the narcoleptic-like sleep structure alterations can slowly recover after trypanocydal therapy, especially when patients are not severely ill (Buguet et al., 1999). This suggests that functional compensation can be effective when the disease is promptly cured.

The present finding of MCH neuron damage shows that T. b. gambiense infection does not affect OX neurons selectively. This also occurs in other conditions. For example, sleep disorders represent prominent non-motor symptoms in Parkinson’s disease, and loss of both OX and MCH neurons, increasing with disease severity, has been reported in post-mortem studies of the hypothalamus of victims of this disease (Thannickal et al., 2007). It is relevant to recall, in this respect, that MCH neurons are instead spared in the brain of narcoleptic patients with or without cataplexy (Peyron et al., 2000; Thannickal et al., 2000, 2009). Altogether the findings indicate that T. b. gambiense infection disrupts the interplay between OX and MCH neurons, supporting data obtained in laboratory rodents after T. b. brucei infection (Palomba et al., 2015). These peptidergic neurons not only play reciprocal roles in the regulation of vigilance states (Konadhode et al., 2015), but are also interconnected. Notably, MCH neurons exert an inhibitory influence on OX neurons, tuning the overall output of these two systems (Rao et al., 2008).

Interestingly, the reduction of OX and MCH neurons here documented in T. b. gambiense infection is much more marked than that provoked by local (intra-hypothalamic) infusion of the endotoxin lipopolysaccharide for 1 month (Gerashchenko and Shiromani, 2004). Experimental studies based on T. b. brucei infection have indicated an escalating inflammatory response during disease progression (Kristensson et al., 2010) in which the posterior hypothalamus is especially involved (Laperchia et al., 2016). Parasites reside in the median eminence, as in other circumventricular organs, since the first stage of hemolymphatic infection (Kristensson et al., 2010). The posterior hypothalamus is an early site of parasite traversal of blood-brain barrier through gradients of permeability from the median-eminence-arcuate nucleus complex (Laperchia et al., 2016). This hypothalamic complex is known to represent a first order station for peripheral signals, transmitting information to the second order network provided by OX and MCH neurons (Guyon et al., 2009; Rostène et al., 2011). It may therefore not be surprising that these peptidergic cell populations are targeted by chronic inflammatory signaling during African trypanosomiasis.

Several data sets point to vulnerability of OX (Grossberg et al., 2011) and MCH (Sergeyev et al., 2001) neurons to inflammatory molecules. OX neurons are especially sensitive to nitric oxide toxicity (Obukuro et al., 2013). MCH neurons are very sensitive to signaling mediated by the CCL2 chemokine (Le Thuc et al., 2016). The expression of this chemokine in the brain during African trypanosomiasis remains to be explored, but CCL2 is part of the panel of inflammatory mediators increased in the CSF of T. b. gambiense HAT patients (Hainard et al., 2009).

In conclusion, the present findings show that sleep-wake-regulatory OX and MCH neurons are vulnerable to the infection caused by a human-pathogenic parasite responsible for the vast majority of HAT cases, and indicate that MCH neurons are especially susceptible to this infection. HAT causes a paradigmatic chronic progressive neuroinflammation, and the present data could therefore have pathogenetic implications for sleep disorders in other chronic neuroinflammatory conditions. Concerning HAT, the data recall the importance of an early diagnosis and therapy to favor compensation and recovery of vulnerable neuronal cell types damaged during the disease.

Author Contributions

CL and Y-ZX: data analysis and manuscript preparation. Y-ZX: tissue processing. DMN: infection design and animal experiments. TC: manuscript preparation: MB: study design and article writing.

Funding

This work was supported by intramural funds at Institut National de Recherche Biomédicale (INRB) and at the University of Verona.

Conflict of Interest Statement

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

References

Belle, M. D., and Piggins, H. D. (2017). Circadian regulation of mouse suprachiasmatic nuclei neuronal states shapes responses to orexin. Eur. J. Neurosci. 45, 723–732. doi: 10.1111/ejn.13506

PubMed Abstract | CrossRef Full Text | Google Scholar

Belle, M. D., Hughes, A. T., Bechtold, D. A., Cunningham, P., Pierucci, M., Burdakov, D., et al. (2014). Acute suppressive and long-term phase modulation actions of orexin on the mammalian circadian clock. J. Neurosci. 34, 3607–3621. doi: 10.1523/jneurosci.3388-13.2014

PubMed Abstract | CrossRef Full Text | Google Scholar

Bhagwandin, A., Fuxe, K., Bennett, N. C., and Manger, P. R. (2011a). Distribution of orexinergic neurons and their terminal networks in the brains of two species of African mole rats. J. Chem. Neuroanat. 41, 32–42. doi: 10.1016/j.jchemneu.2010.11.002

PubMed Abstract | CrossRef Full Text | Google Scholar

Bhagwandin, A., Gravett, N., Hemingway, J., Oosthuizen, M. K., Bennett, N. C., Siegel, J. M., et al. (2011b). Orexinergic neuron numbers in three species of African mole rats with rhythmic and arrhythmic chronotypes. Neuroscience 199, 153–165. doi: 10.1016/j.neuroscience.2011.10.023

PubMed Abstract | CrossRef Full Text | Google Scholar

Bittencourt, J. C. (2011). Anatomical organization of the melanin-concentrating hormone peptide family in the mammalian brain. Gen. Comp. Endocrinol. 172, 185–197. doi: 10.1016/j.ygcen.2011.03.028

PubMed Abstract | CrossRef Full Text | Google Scholar

Blum, J., Schmid, C., and Burri, C. (2006). Clinical aspects of 2541 patients with second stage human African trypanosomiasis. Acta Trop. 97, 55–64. doi: 10.1016/j.actatropica.2005.08.001

PubMed Abstract | CrossRef Full Text | Google Scholar

Bourgin, P., Zeitzer, J. M., and Mignot, E. (2008). CSF hypocretin-1 assessment in sleep and neurological disorders. Lancet Neurol. 7, 649–662. doi: 10.1016/s1474-4422(08)70140-6

PubMed Abstract | CrossRef Full Text | Google Scholar

Buguet, A., Bisser, S., Josenando, T., Chapotot, F., and Cespuglio, R. (2005). Sleep structure: a new diagnostic tool for stage determination in sleeping sickness. Acta Trop. 93, 107–117. doi: 10.1016/j.actatropica.2004.10.001

PubMed Abstract | CrossRef Full Text | Google Scholar

Buguet, A., Bourdon, L., Bisser, S., Chapotot, F., Radomski, M. W., and Dumas, M. (2001). Sleeping sickness: major disorders of circadian rhythm. Med. Trop. 61, 328–339.

PubMed Abstract | Google Scholar

Buguet, A., Mpanzou, G., and Bentivoglio, M. (2014). “Human African trypanosomiasis: a highly neglected neurological disease,” in Neglected Tropical Diseases and Conditions of the Nervous System, eds M. Bentivoglio, E. A. Cavalheiro, K. Kristensson and N. B. Patel (New York, NY: Springer-Verlag), 165–181.

Google Scholar

Buguet, A., Tapie, P., and Bert, J. (1999). Reversal of the sleep/wake cycle disorder of sleeping sickness after trypanosomicide treatment. J. Sleep Res. 8, 225–235. doi: 10.1046/j.1365-2869.1999.00160.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Büscher, P., Bin Shamamba, S. K., Ngoyi, D. M., Pyana, P., Baelmans, R., Magnus, E., et al. (2005). Susceptibility of Grammomys surdaster thicket rats to Trypanosoma brucei gambiense infection. Trop. Med. Int. Health 10, 850–855. doi: 10.1111/j.1365-3156.2005.01468.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Büscher, P., Cecchi, G., Jamonneau, V., and Priotto, G. (2017). Human African trypanosomiasis. Lancet 390, 2397–2409. doi: 10.1016/S0140-6736(17)31510-6

PubMed Abstract | CrossRef Full Text | Google Scholar

Coetzee, C. G. (1975). The biology, behaviour and ecology of Mastomys natalensis in southern Africa. Bull. World Health Organ. 52, 637–644.

PubMed Abstract | Google Scholar

Colavito, V., Tesoriero, C., Wirtu, A. T., Grassi-Zucconi, G., and Bentivoglio, M. (2015). Limbic thalamus and state-dependent behavior: the paraventricular nucleus of the thalamic midline as a node in circadian timing and sleep/wake-regulatory networks. Neurosci. Biobehav. Rev. 54, 3–17. doi: 10.1016/j.neubiorev.2014.11.021

PubMed Abstract | CrossRef Full Text | Google Scholar

Dantz, B., Edgar, D. M., and Dement, W. C. (1994). Circadian rhythms in narcolepsy: studies on a 90 minute day. Electroencephalogr. Clin. Neurophysiol. 90, 24–35. doi: 10.1016/0013-4694(94)90110-4

PubMed Abstract | CrossRef Full Text | Google Scholar

Darsaud, A., Bourdon, L., Chevrier, C., Keita, M., Bouteille, B., Queyroy, A., et al. (2003). Clinical follow-up in the rat experimental model of African trypanosomiasis. Exp. Biol. Med. 228, 1355–1362. doi: 10.1177/153537020322801114

PubMed Abstract | CrossRef Full Text | Google Scholar

Dauvilliers, Y., Bisser, S., Chapotot, F., Vatunga, G., Cespuglio, R., Josenando, T., et al. (2008). Hypocretin and human African trypanosomiasis. Sleep 31, 348–354.

PubMed Abstract | Google Scholar

de Lecea, L., and Huerta, R. (2014). Hypocretin (orexin) regulation of sleep-to-wake transitions. Front. Pharmacol. 5:16. doi: 10.3389/fphar.2014.00016

PubMed Abstract | CrossRef Full Text | Google Scholar

Ferreira, J. G. P., Duarte, J. C. G., Diniz, G. B., and Bittencourt, J. C. (2017). Litter size determines the number of melanin-concentrating hormone neurons in the medial preoptic area of Sprague Dawley lactating dams. Physiol. Behav. 181, 75–79. doi: 10.1016/j.physbeh.2017.08.028

PubMed Abstract | CrossRef Full Text | Google Scholar

Gerashchenko, D., Murillo-Rodriguez, E., Lin, L., Xu, M., Hallett, L., Nishino, S., et al. (2003). Relationship between CSF hypocretin levels and hypocretin neuronal loss. Exp. Neurol. 184, 1010–1016. doi: 10.1016/s0014-4886(03)00388-1

PubMed Abstract | CrossRef Full Text | Google Scholar

Gerashchenko, D., and Shiromani, P. J. (2004). Effects of inflammation produced by chronic lipopolysaccharide administration on the survival of hypocretin neurons and sleep. Brain Res. 1019, 162–169. doi: 10.1016/j.brainres.2004.06.016

PubMed Abstract | CrossRef Full Text | Google Scholar

Giroud, C., Ottones, F., Coustou, V., Dacheux, D., Biteau, N., Miezan, B., et al. (2009). Murine Models for Trypanosoma brucei gambiense disease progression—from silent to chronic infections and early brain tropism. PLoS Negl. Trop. Dis. 3:e509. doi: 10.1371/journal.pntd.0000509

PubMed Abstract | CrossRef Full Text | Google Scholar

Golombek, D. A., and Rosenstein, R. E. (2010). Physiology of circadian entrainment. Physiol. Rev. 90, 1063–1102. doi: 10.1152/physrev.00009.2009

PubMed Abstract | CrossRef Full Text | Google Scholar

Grossberg, A. J., Zhu, X., Leinninger, G. M., Levasseur, P. R., Braun, T. P., Myers, M. G. Jr., et al. (2011). Inflammation-induced lethargy is mediated by suppression of orexin neuron activity. J. Neurosci. 31, 11376–11386. doi: 10.1523/jneurosci.2311-11.2011

PubMed Abstract | CrossRef Full Text | Google Scholar

Guyon, A., Conductier, G., Rovere, C., Enfissi, A., and Nahon, J. L. (2009). Melanin-concentrating hormone producing neurons: activities and modulations. Peptides 30, 2031–2039. doi: 10.1016/j.peptides.2009.05.028

PubMed Abstract | CrossRef Full Text | Google Scholar

Hainard, A., Tiberti, N., Robin, X., Lejon, V., Ngoyi, D. M., Matovu, E., et al. (2009). A combined CXCL10, CXCL8 and H-FABP panel for the staging of human African trypanosomiasis patients. PLoS Negl. Trop. Dis. 3:e459. doi: 10.1371/journal.pntd.0000459

PubMed Abstract | CrossRef Full Text | Google Scholar

Isaäcson, M. (1975). The ecology of Praomys (Mastomys) natalensis in southern Africa. Bull. World Health Organ. 52, 629–636.

PubMed Abstract | Google Scholar

Kennedy, P. G. (2013). Clinical features, diagnosis, and treatment of human African trypanosomiasis (sleeping sickness). Lancet Neurol. 12, 186–194. doi: 10.1016/S1474-4422(12)70296-X

PubMed Abstract | CrossRef Full Text | Google Scholar

Kirouac, G. J., Parsons, M. P., and Li, S. (2005). Orexin (hypocretin) innervation of the paraventricular nucleus of the thalamus. Brain Res. 1059, 179–188. doi: 10.1016/j.brainres.2005.08.035

PubMed Abstract | CrossRef Full Text | Google Scholar

Konadhode, R. R., Pelluru, D., and Shiromani, P. J. (2015). Neurons containing orexin or melanin concentrating hormone reciprocally regulate wake and sleep. Front. Syst. Neurosci. 8:244. doi: 10.3389/fnsys.2014.00244

PubMed Abstract | CrossRef Full Text | Google Scholar

Kristensson, K., Nygård, M., Bertini, G., and Bentivoglio, M. (2010). African trypanosome infections of the nervous system: parasite entry and effects on sleep and synaptic functions. Prog. Neurobiol. 91, 152–171. doi: 10.1016/j.pneurobio.2009.12.001

PubMed Abstract | CrossRef Full Text | Google Scholar

Laperchia, C., Palomba, M., Seke Etet, P. F., Rodgers, J., Bradley, B., Montague, P., et al. (2016). Trypanosoma brucei invasion and T-cell infiltration of the brain parenchyma in experimental sleeping sickness: timing and correlation with functional changes. PLoS Negl. Trop. Dis. 10:e0005242. doi: 10.1371/journal.pntd.0005242

PubMed Abstract | CrossRef Full Text | Google Scholar

Laperchia, C., Tesoriero, C., Seke-Etet, P. F., La Verde, V., Colavito, V., Grassi-Zucconi, G., et al. (2017). Expression of interferon-inducible chemokines and sleep/wake changes during early encephalitis in experimental African trypanosomiasis. PLoS Negl. Trop. Dis. 11:e0005854. doi: 10.1371/journal.pntd.0005854

PubMed Abstract | CrossRef Full Text | Google Scholar

Le Thuc, O., Cansell, C., Bourourou, M., Denis, R. G., Stobbe, K., Devaux, N., et al. (2016). Central CCL2 signaling onto MCH neurons mediates metabolic and behavioral adaptation to inflammation. EMBO Rep. 17, 1738–1752. doi: 10.15252/embr.201541499

PubMed Abstract | CrossRef Full Text | Google Scholar

Lejon, V., Bentivoglio, M., and Franco, J. R. (2013). Human African trypanosomiasis. Handb. Clin. Neurol. 114, 169–181. doi: 10.1016/B978-0-444-53490-3.00011-X

PubMed Abstract | CrossRef Full Text | Google Scholar

Lhermitte, J. (1910). La Maladie du Sommeil et Les Narcolepsies. Bruxelles: Etablissements D’imprimerie L. Severeyns.

Li, S. B., Jones, J. R., and de Lecea, L. (2016). Hypocretins, neural systems, physiology, and psychiatric disorders. Curr. Psychiatry Rep. 18:7. doi: 10.1007/s11920-015-0639-0

PubMed Abstract | CrossRef Full Text | Google Scholar

Liblau, R. S., Vassalli, A., Seifinejad, A., and Tafti, M. (2015). Hypocretin (orexin) biology and the pathophysiology of narcolepsy with cataplexy. Lancet Neurol. 14, 318–328. doi: 10.1016/S1474-4422(14)70218-2

PubMed Abstract | CrossRef Full Text | Google Scholar

Marston, O. J., Williams, R. H., Canal, M. M., Samuels, R. E., Upton, N., and Piggins, H. D. (2008). Circadian and dark-pulse activation of orexin/hypocretin neurons. Mol. Brain 1:19. doi: 10.1186/1756-6606-1-19

PubMed Abstract | CrossRef Full Text | Google Scholar

McGranaghan, P. A., and Piggins, H. D. (2001). Orexin A-like immunoreactivity in the hypothalamus and thalamus of the Syrian hamster (Mesocricetus auratus) and Siberian hamster (Phodopus sungorus), with special reference to circadian structures. Brain Res. 904, 234–244. doi: 10.1016/s0006-8993(01)02463-5

PubMed Abstract | CrossRef Full Text | Google Scholar

Mehlitz, D. (1975). Serological studies on subgenus-differentiation and persistence of antibodies following infections with Trypanosomes (author’s transl). Tropenmed. Parasitol. 26, 265–275.

PubMed Abstract | Google Scholar

Mehlitz, D. (1978). Investigations on the susceptibility of Mastomys natalensis to Trypanosoma (trypanozoon) brucei gambiense (author’s transl). Tropenmed. Parasitol. 29, 101–107.

PubMed Abstract | Google Scholar

Mesu, V. K. B. K., Kalonji, W. M., Bardonneau, C., Mordt, O. V., Blesson, S., Simon, F., et al. (2018). Oral fexinidazole for late-stage African Trypanosoma brucei gambiense trypanosomiasis: a pivotal multicentre, randomised, non-inferiority trial. Lancet 391, 144–154. doi: 10.1016/S0140-6736(17)32758-7

PubMed Abstract | CrossRef Full Text | Google Scholar

Mintz, E. M., van den Pol, A. N., Casano, A. A., and Albers, H. E. (2001). Distribution of hypocretin-(orexin) immunoreactivity in the central nervous system of Syrian hamsters (Mesocricetus auratus). J. Chem. Neuroanat. 21, 225–238. doi: 10.1016/s0891-0618(01)00111-9

PubMed Abstract | CrossRef Full Text | Google Scholar

Moore, R. Y. (2013). The suprachiasmatic nucleus and the circadian timing system. Prog. Mol. Biol. Transl. Sci. 119, 1–28. doi: 10.1016/b978-0-12-396971-2.00001-4

PubMed Abstract | CrossRef Full Text | Google Scholar

Mulungu, L. S., Ngowo, V., Mdangi, M., Katakweba, A. S., Tesha, P., Mrosso, F. P., et al. (2013). Population dynamics and breeding patterns of multimammate mouse, Mastomys natalensis (Smith 1834), in irrigated rice fields in eastern Tanzania. Pest Manag. Sci. 69, 371–377. doi: 10.1002/ps.3346

PubMed Abstract | CrossRef Full Text | Google Scholar

Nixon, J. P., and Smale, L. (2007). A comparative analysis of the distribution of immunoreactive orexin A and B in the brains of nocturnal and diurnal rodents. Behav. Brain Funct. 3:28. doi: 10.1186/1744-9081-3-28

PubMed Abstract | CrossRef Full Text | Google Scholar

Obukuro, K., Nobunaga, M., Takigawa, M., Morioka, H., Hisatsune, A., Isohama, Y., et al. (2013). Nitric oxide mediates selective degeneration of hypothalamic orexin neurons through dysfunction of protein disulfide isomerase. J. Neurosci. 33, 12557–12568. doi: 10.1523/JNEUROSCI.0595-13.2013

PubMed Abstract | CrossRef Full Text | Google Scholar

Palomba, M., Seke-Etet, P. F., Laperchia, C., Tiberio, L., Xu, Y. Z., Colavito, V., et al. (2015). Alterations of orexinergic and melanin-concentrating hormone neurons in experimental sleeping sickness. Neuroscience 290, 185–195. doi: 10.1016/j.neuroscience.2014.12.066

PubMed Abstract | CrossRef Full Text | Google Scholar

Pardridge, W. M., Boado, R. J., and Farrell, C. R. (1990). Brain-type glucose transporter (GLUT-1) is selectively localized to the blood-brain barrier. Studies with quantitative western blotting and in situ hybridization. J. Biol. Chem. 265, 18035–18040.

PubMed Abstract | Google Scholar

Peng, Z. C., Chen, S., and Bentivoglio, M. (1995). A sensitive double immunostaining protocol for Fos-immunoreactive neurons. Brain Res. Bull. 36, 101–105. doi: 10.1016/0361-9230(94)00125-k

PubMed Abstract | CrossRef Full Text | Google Scholar

Peyron, C., Faraco, J., Rogers, W., Ripley, B., Overeem, S., Charnay, Y., et al. (2000). A mutation in a case of early onset narcolepsy and a generalized absence of hypocretin peptides in human narcoleptic brains. Nat. Med. 6, 991–997. doi: 10.1038/79690

PubMed Abstract | CrossRef Full Text | Google Scholar

Peyron, C., Tighe, D. K., van den Pol, A. N., de Lecea, L., Heller, H. C., Sutcliffe, J. G., et al. (1998). Neurons containing hypocretin (orexin) project to multiple neuronal systems. J. Neurosci. 18, 9996–10015.

PubMed Abstract | Google Scholar

Poon, D. C., Ho, Y. S., Chiu, K., Wong, H. L., and Chang, R. C. (2015). Sickness: from the focus on cytokines, prostaglandins and complement factors to the perspectives of neurons. Neurosci. Biobehav. Rev. 57, 30–45. doi: 10.1016/j.neubiorev.2015.07.015

PubMed Abstract | CrossRef Full Text | Google Scholar

Rao, Y., Lu, M., Ge, F., Marsh, D. J., Qian, S., Wang, A. H., et al. (2008). Regulation of synaptic efficacy in hypocretin/orexin-containing neurons by melanin concentrating hormone in the lateral hypothalamus. J. Neurosci. 28, 9101–9110. doi: 10.1523/JNEUROSCI.1766-08.2008

PubMed Abstract | CrossRef Full Text | Google Scholar

Rostène, W., Dansereau, M. A., Godefroy, D., Van Steenwinckel, J., Reaux-Le Goazigo, A., Melik-Parsadaniantz, S., et al. (2011). Neurochemokines: a menage a trois providing new insights on the functions of chemokines in the central nervous system. J. Neurochem. 118, 680–694. doi: 10.1111/j.1471-4159.2011.07371.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Sakurai, T. (2014). Roles of orexins in the regulation of body weight homeostasis. Obes. Res. Clin. Pract. 8, e414–e420. doi: 10.1016/j.orcp.2013.12.001

PubMed Abstract | CrossRef Full Text | Google Scholar

Saper, C. B., Fuller, P. M., Pedersen, N. P., Lu, J., and Scammell, T. E. (2010). Sleep state switching. Neuron 68, 1023–1042. doi: 10.1016/j.neuron.2010.11.032

PubMed Abstract | CrossRef Full Text | Google Scholar

Sateia, M. J. (2014). International classification of sleep disorders-third edition: highlights and modifications. Chest 146, 1387–1394. doi: 10.1378/chest.14-0970

PubMed Abstract | CrossRef Full Text | Google Scholar

Scammell, T. E. (2015). Narcolepsy. N. Engl. J. Med. 373, 2654–2662. doi: 10.1056/NEJMra1500587

PubMed Abstract | CrossRef Full Text | Google Scholar

Scammell, T. E., Arrigoni, E., and Lipton, J. O. (2017). Neural circuitry of wakefulness and sleep. Neuron 93, 747–765. doi: 10.1016/j.neuron.2017.01.014

PubMed Abstract | CrossRef Full Text | Google Scholar

Seke Etet, P. F., Palomba, M., Colavito, V., Grassi-Zucconi, G., Bentivoglio, M., and Bertini, G. (2012). Sleep and rhythm changes at the time of Trypanosoma brucei invasion of the brain parenchyma in the rat. Chronobiol. Int. 29, 469–481. doi: 10.3109/07420528.2012.660713

PubMed Abstract | CrossRef Full Text | Google Scholar

Sergeyev, V., Broberger, C., and Hökfelt, T. (2001). Effect of LPS administration on the expression of POMC, NPY, galanin, CART and MCH mRNAs in the rat hypothalamus. Mol. Brain Res. 90, 93–100. doi: 10.1016/s0169-328x(01)00088-2

PubMed Abstract | CrossRef Full Text | Google Scholar

Sweigers, J., Bhagwandin, A., Spocter, M. A., Kaswera-Kyamakya, C., Gilissen, E., Manger, P. R., et al. (2017). Nuclear organisation of cholinergic, catecholaminergic, serotonergic and orexinergic neurons in two relatively large-brained rodent species-The springhare (Pedetes capensis) and Beecroft’s scaly-tailed squirrel (Anomalurus beecrofti). J. Chem. Neuroanat. 86, 78–91. doi: 10.1016/j.jchemneu.2017.09.002

PubMed Abstract | CrossRef Full Text | Google Scholar

Tesoriero, C., Xu, Y.-Z., Mumba Ngoyi, D., and Bentivoglio, M. (2018). Neural damage in experimental Trypanosoma brucei gambiense infection: the suprachiasmatic nucleus. Front. Neuroanat. doi: 10.3389/fnana.2018.00006 [Epub ahead of print].

CrossRef Full Text | Google Scholar

Thannickal, T. C., Lai, Y. Y., and Siegel, J. M. (2007). Hypocretin (orexin) cell loss in Parkinson’s disease. Brain 130, 1586–1595. doi: 10.1093/brain/awm097

PubMed Abstract | CrossRef Full Text | Google Scholar

Thannickal, T. C., Moore, R. Y., Nienhuis, R., Ramanathan, L., Gulyani, S., Aldrich, M., et al. (2000). Reduced number of hypocretin neurons in human narcolepsy. Neuron 27, 469–474. doi: 10.1016/s0896-6273(00)00058-1

PubMed Abstract | CrossRef Full Text | Google Scholar

Thannickal, T. C., Nienhuis, R., and Siegel, J. M. (2009). Localized loss of hypocretin (orexin) cells in narcolepsy without cataplexy. Sleep 32, 993–998. doi: 10.1093/sleep/32.8.993

PubMed Abstract | CrossRef Full Text | Google Scholar

Torterolo, P., Scorza, C., Lagos, P., Urbanavicius, J., Benedetto, L., Pascovich, C., et al. (2015). Melanin-concentrating hormone (MCH): role in REM sleep and depression. Front. Neurosci. 9:475. doi: 10.3389/fnins.2015.00475

PubMed Abstract | CrossRef Full Text | Google Scholar

van Esseveldt, K. E., Lehman, M. N., and Boer, G. J. (2000). The suprachiasmatic nucleus and the circadian time-keeping system revisited. Brain Res. Brain Res. Rev. 33, 34–77. doi: 10.1016/s0165-0173(00)00025-4

PubMed Abstract | CrossRef Full Text | Google Scholar

Welburn, S. C., Molyneux, D. H., and Maudlin, I. (2016). Beyond tsetse—implications for research and control of human african trypanosomiasis epidemics. Trends Parasitol. 32, 230–241. doi: 10.1016/j.pt.2015.11.008

PubMed Abstract | CrossRef Full Text | Google Scholar

WHO. (2017). Trypanosomiasis, Human African (Sleeping Sickness) [Online]. Fact sheet/c N. 259. Available online at: http://www.who.int/mediacentre/factsheets/fs259/en/

Keywords: human African trypanosomiasis, orexin, hypocretin, melanin-concentrating hormone, neuroinflammation, sleep, wake

Citation: Laperchia C, Xu Y-Z, Mumba Ngoyi D, Cotrufo T and Bentivoglio M (2018) Neural Damage in Experimental Trypanosoma brucei gambiense Infection: Hypothalamic Peptidergic Sleep and Wake-Regulatory Neurons. Front. Neuroanat. 12:13. doi: 10.3389/fnana.2018.00013

Received: 07 December 2017; Accepted: 07 February 2018;
Published: 27 February 2018.

Edited by:

Nouria Lakhdar-Ghazal, Mohammed V University, Morocco

Reviewed by:

Jackson Cioni Bittencourt, University of São Paulo, Brazil
Khalid El Allali, Institut Agronomique et Vétérinaire Hassan II, Morocco

Copyright © 2018 Laperchia, Xu, Mumba Ngoyi, Cotrufo and Bentivoglio. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.

*Correspondence: Marina Bentivoglio, marina.bentivoglio@univr.it

Present address: Claudia Laperchia, Department of Fundamental Neurosciences, Faculty of Biology and Medicine, University of Lausanne, Lausanne, Switzerland
Yuan-Zhong Xu, Brown Foundation Institute of Molecular Medicine, University of Texas Health Science Center, Houston, TX, United States
Tiziana Cotrufo, Department of Cell Biology, Physiology and Immunology, Faculty of Biology, University of Barcelona, Barcelona, Spain