ORIGINAL RESEARCH article
Volume 11 - 2017 | https://doi.org/10.3389/fnins.2017.00437
Cell Proliferation, Migration, and Neurogenesis in the Adult Brain of the Pulse Type Weakly Electric Fish, Gymnotus omarorum
- 1Desarrollo y Evolución Neural, Departamento de Neurociencias Integrativas y Computacionales, Instituto de Investigaciones Biológicas Clemente Estable, Ministerio de Educación y Cultura, Montevideo, Uruguay
- 2Departamento de Histología y Embriología, Facultad de Medicina, Universidad de la República, Montevideo, Uruguay
- 3IIBE “Histología de Sistemas Sensoriales”, Unidad Asociada F. de Medicina, Montevideo, Uruguay
Adult neurogenesis, an essential mechanism of brain plasticity, enables brain development along postnatal life, constant addition of new neurons, neuronal turnover, and/or regeneration. It is amply distributed but negatively modulated during development and along evolution. Widespread cell proliferation, high neurogenic, and regenerative capacities are considered characteristics of teleost brains during adulthood. These anamniotes are promising models to depict factors that modulate cell proliferation, migration, and neurogenesis, and might be intervened to promote brain plasticity in mammals. Nevertheless, the migration path of derived cells to their final destination was not studied in various teleosts, including most weakly electric fish. In this group adult brain morphology is attributed to sensory specialization, involving the concerted evolution of peripheral electroreceptors and electric organs, encompassed by the evolution of neural networks involved in electrosensory information processing. In wave type gymnotids adult brain morphology is proposed to result from lifelong region specific cell proliferation and neurogenesis. Consistently, pulse type weakly electric gymnotids and mormyrids show widespread distribution of proliferation zones that persists in adulthood, but their neurogenic potential is still unknown. Here we studied the migration process and differentiation of newborn cells into the neuronal phenotype in the pulse type gymnotid Gymnotus omarorum. Pulse labeling of S-phase cells with 5-Chloro-2′-deoxyuridine thymidine followed by 1 to 180 day survivals evidenced long distance migration of newborn cells from the rostralmost telencephalic ventricle to the olfactory bulb, and between layers of all cerebellar divisions. Shorter migration appeared in the tectum opticum and torus semicircularis. In many brain regions, derived cells expressed early neuronal markers doublecortin (chase: 1–30 days) and HuC/HuD (chase: 7–180 days). Some newborn cells expressed the mature neuronal marker tyrosine hydroxylase in the subpallium (chase: 90 days) and olfactory bulb (chase: 180 days), indicating the acquisition of a mature neuronal phenotype. Long term CldU labeled newborn cells of the granular layer of the corpus cerebelli were also retrogradely labeled “in vivo,” suggesting their insertion into the neural networks. These findings evidence the neurogenic capacity of telencephalic, mesencephalic, and rhombencephalic brain proliferation zones in G. omarorum, supporting the phylogenetic conserved feature of adult neurogenesis and its functional significance.
Neurogenesis is the main mechanism of adult brain plasticity that enables the continuation of brain development, the constant addition of new neurons and/or the neuronal turnover (Barker et al., 2011; Alunni and Bally-Cuif, 2016). It has been demonstrated in a wide range of animals, from cnidarians to mammals, including humans (Altman, 1963, 1969; Altman and Das, 1965; Sullivan et al., 2007; Galliot and Quiquand, 2011). Neurogenesis is progressively restricted during animal development and negatively modulated along evolution. Its spatial distribution remains widespread in all brain divisions of adult anamniotes, particularly in teleost fish (Cayre et al., 2002; Lindsey and Tropepe, 2006; Kaslin et al., 2008; Barker et al., 2011; Grandel and Brand, 2013). However, it is almost confined to two zones in the telencephalon of adult mammals (Ma et al., 2008; Altman, 2011; Vadodaria and Gage, 2014).
Soon after the discovery of adult neurogenesis in mammals by Altman (Altman, 1962, 1963; Altman and Das, 1965, 1966) the widespread distribution of cell proliferation in the brain of adult teleost was evidenced by tritiated thymidine (3H-thymidine) labeling (Brachydanio rerio: Rahmann, 1968; Lebistes reticulatus: Richter and Kranz, 1970). In spite of ultrastructural evidences of adult neurogenesis in mammals (Kaplan and Hinds, 1977), the field of cell proliferation and neurogenesis in both amniotes and anamniotes resumed after a 20 years hindrance (Gross, 2000). Even though the spatial distribution of proliferation zones was since then evidenced in several teleost, numerous taxa remain underexplored. One of the earliest and most thoroughly studied anamniotes is the wave type weakly electric gymnotid Apteronotus leptorhynchus, which is considered a classical biological model in the field. Weakly electric fish are also good models for the study of brain evolution sub-serving variations in animal behavior (Albert et al., 1998). The peculiar adult brain morphology of weakly electric fish is associated to the relevance of the electrosensory modality for these fish lifestyle (Evans, 1940; Bennett, 1971; Hodos and Butler, 1997; Kotrschal et al., 1998; Meek and Nieuwenhuys, 1998; Ito et al., 2007; Shumway, 2008). It results from the differential growth of portions of the neural tube that progressively differentiate into brain vesicles followed by the subsequent formation and differential growth of brain structures derived from the alar plate, as shown in wave (Leyhausen et al., 1987; Lannoo et al., 1990) and pulse (Iribarne and Castelló, 2014) gymnotids, and pulse mormyrids (Haugedé-Carré et al., 1977, 1979; Radmilovich et al., 2016). The maintenance of adult brain morphology as fish body grows indefinitely depends in turn on heterogeneous cell proliferation and neurogenesis. Thus, neurogenesis can be considered as a plastic mechanism to maintain the “proper mass” of neural tissue controlling particular functions (Jerisson, 1973) or for the “matching” between peripheral elements and brain processing power (Zupanc, 2006, 2008, 2011), contributing to the functional specialization (Grandel et al., 2006). Brain proliferation zones also persist in adulthood in G. omarorum (Olivera-Pasilio et al., 2014) and Brachyhypopomus gauderio (Dunlap et al., 2011) showing overall similarities with their distribution in A. leptorhynchus (Zupanc and Horschke, 1995; Zupanc, 2006, 2008).
Adult G. omarorum newborn cells appear to differ in their pace of migration (Olivera-Pasilio et al., 2014). Newborn cells show long distance displacement at the rostral part of the telencephalon, suggesting a migration process similar to what occurs in amniotes (Altman, 1969; Lim et al., 2008) including humans (Wang et al., 2011) and birds (Goldman and Nottebohm, 1983; Nottebohm, 2002; Barnea and Pravosudov, 2011), and anamniotes (Danio rerio: Adolf et al., 2006; Kishimoto et al., 2011). Other brain region of comparative interest are the cerebellum (Cb), the dorsal, ventral, and posterior subdivisions of the dorsolateral zone of the dorsal telencephalon (considered homologous of the amniote hippocampus; Zupanc, 2006) and the tectum opticum (TeO). Newborn cells originated from these proliferation zones also display long range and/or relatively fast migration, as evidenced by the almost complete displacement of derived cells between cerebellar layers after a 30 days chase (Olivera-Pasilio et al., 2014). The location, as well as shape and appearance of the nuclei suggest that newborn cells are in the process of differentiation as shown in other teleost (Zupanc et al., 1996, 2005; Kaslin et al., 2009; Delgado and Schmachtenberg, 2011; Teles et al., 2012).
In this manuscript, we further analyze in adult G. omarorum the migration process of derived cells by pursuing their location from the proliferation zones to their final destination. We also studied the differentiation of newborn cells into the neuronal phenotype by demonstrating the co-localization of long-term thymidine analog labeling and expression of early neuronal markers doublecortin (DCX) and HuC/HuD or the mature neuronal marker tyrosine hydroxylase (TH). We found evidences of neurogenesis in several brain regions of the telencephalon, mesencephalon, and rhombencephalon. We further evidenced the insertion of newborn cells into neural circuits by the demonstration of long term thymidine analog labeling and “in vivo” retrogradely labeling of cerebellar granular cells. These findings contribute to support the widespread distribution of brain proliferation zones and their neurogenic capacity in teleost.
Materials and Methods
Thirteen adult specimens of G. omarorum (Richer-de-Forges et al., 2009; 8 males, 2 females and 3 of non-determined sex; weight: 6.26 ± 2.94; total fish length: 12.23 ± 2.04 mean ± SD) were collected from Laguna del Cisne, Uruguay (latitude 35°50 S, longitude 55°08 W). According to the measured length of the specimens, which is about half of the maximal length (Richer-de-Forges et al., 2009), we estimate that most of the fish used in this study have already reached the adult period, corresponding to the first gonadal maturation, at the age of 1 year (Balon, 1975; Barbieri and Cruz, 1983).
Macroscopic gonadal morphology was confirmed in 10 of the specimens studied. Animals were kept in individual tanks on a 12 h:12 h light: dark cycle and daily fed with Tubifex tubifex. Water conductivity was adjusted to 200 μs and temperature maintained at 20–25°C.
All procedures were performed in accordance to the guidelines of CHEA (Comisión Honoraria de Experimentación Animal, ordinance number: 4332-99, Universidad de la República). Experiments were approved by the Animal Ethics Committee of the Instituto de Investigaciones Biológicas Clemente Estable (protocol number 010/09/2011).
For the application of Neurobiotin tracer (Vector Laboratories, Burlingame, CA, USA) in the corpus cerebelli (CCb), animals were anesthetized by immersion in 3-aminobenzoic acid ethyl ester (MS-222, Sigma-Aldrich, St Louis, MO, USA, at a dose of 120 mg/l) maintained by gill perfusion of the same anesthetic solution during surgery.
For transcardial fixation, fish were deeply anesthetized by immersion in MS-222 (500 mg/l, Sigma-Aldrich) followed by gill perfusion of the same anesthetic solution.
Fixation and Tissue Sectioning
Animals were first perfused with 20–30 ml of saline (0.7% NaCl solution) in order to wash blood out from the circulatory system, followed by 10% paraformaldehyde (Sigma-Aldrich) dissolved in phosphate buffer 0.1 M, pH 7.4 (PB; Carlo Erba, Val de Reuil, France). Brains were dissected out and post fixed in the same fixative solution for 24 h at 4°C. After embedding the brains in a gelatin/albumin (Sigma-Aldrich) mixture denatured with glutaraldehyde (Sigma-Aldrich), frontal serial sections (60 μm) were obtained with a vibratome (Leica VT1000S, Wetzlar, Germany) and serially collected in 24 or 48 multiwell plates.
In many cases, sections from most brain regions were processed in parallel, though we focused on certain rostral-caudal levels. At these levels, long distance and/or high pace of migration of newborn cells were previously evidenced (Olivera-Pasilio et al., 2014): the medial (L1) and caudal region (L2) of OB, corresponding to plates 1 of Gymnotus carapo atlas (Corrêa et al., 1998) and plate 38 of A. lepthorhynchyus atlas (Maler et al., 1991); the rostral region of the subpallium (L3) that corresponds to plates 2 and 32 of the mentioned atlases, respectively; the medial region and caudal pole of the midbrain TeO and torus semicircularis (TS; L4, and L5), the rostral pole of the rhombencephalic corpus cerebelli (CCb; L5), and the caudal pole of the rhombencephalic electrosensory lateral line lobe (ELL; L6; Figure 1).
Figure 1. Spatial-temporal distribution of brain labeled cells in adult G. omarorum after short (1 day) and long (30 days) survivals following CldU administration. Labeled cells are qualitatively represented by red and blue dots (after chases of 1 day and 30 days, respectively) in the schematic diagrams of frontal sections (L1–L6) corresponding to the planes indicated by the dotted lines over the lateral view of the brain. Regions of interest of this work are indicated by the green squares. Modified from Olivera-Pasilio et al. (2014). CCb-mol, Cerebellum, molecular layer; CCb, Corpus cerebelli; CP, Central-posterior nucleus; CMS, Centromedial segment; DFl, Nucleus diffusus lateralis of the inferior lobe; EGa, EGa-gra, Eminentia granularis pars anterior, granular layer; ELL, Electrosensory lateral line lobe; eTS, Torus semicircularis efferents; Hv, Hypothalamus ventralis; ICL, Internal cell layer; IL, Inferior lobe; DM1, Dorsomedial telencephalon; DLd, Dorsolateral telencephalon, dorsal subdivision; DM1, Dorsomedial telencephalon, subdivision 1; DM2, Dorsomedial telencephalon, subdivision 2; MgN, Magnocellular mesencephalic nucleus; MS, Medial segment; mol, Molecular layer (ELL); PPn, Prepacemaker nucleus; RF, Reticular formation; TA, Nucleus tuberis anterior; TEL, Telencephalon; TeO, Tectum Opticum; TL, Torus longitudinalis; TPP, Periventricular nucleus of the posterior tuberculum; tStF, Tractus stratum fibrosum; V, Ventricle; Vd, Ventral telencephalon, dorsal subdivision; Vv, Ventral telencephalon, ventral subdivision. Scale bars: 1 mm.
Histological Analysis of the Brain of G. omarorum
To reveal the structural organization of the brain regions under analysis, mainly those where newborn neurons migrate, some sections were counterstained with DAPI (Sigma) or ToPro3 (Molecular Probes, Grand Island, NY, USA) after immunohistochemistry. Also, serial sections of control animals (N = 2) were counterstained with fluorescent Nissl staining using Neuro Trace® (Molecular Probes) as described below (Supplementary Figure 1) and βIII-tubulin, HuC/HuD or tyrosine hydroxylase (TH; Supplementary Figure 2). For fluorescent Nissl counterstaining, free floating brain sections of a control animal were stained with Neuro Trace® at 1/150 dilution in PB for 20 min at room temperature and rinsed in PB with 0.1% Triton X-100 (10 min) followed by PB (3 × 5 min). For ToPro3 counterstaining, brain sections were immersed in ToPro3 for 10 min at a 1/4,000 dilution, followed by rinsing in PB (3 × 5 min). All sections were mounted in a sealing and anti-fading coverslipping solution containing polyvinyl alcohol (PVA, Sigma) and 1,4 diazabicyclo [2.2.2]octane (DABCO, Sigma) and prepared according Peterson lab protocol (http://neurorenew.com/wp-content/uploads/2014/12/pva2.pdf).
In order to evidence the migration and/or differentiation of newborn cells into the neuronal phenotype, we labeled derived cells using two protocols of thymidine analog administration. Then, we demonstrated their differentiation into the neuronal phenotype by demonstration of analog retention by CldU immunohistochemistry combined with immunohistochemical demonstration of neuronal markers' expression or labeling with neuronal tracers.
Thymidine Analog Labeling
Proliferating cells were labeled with 2.3 mg/ml 5-Chloro-2′-deoxyuridine thymidine (CldU, Sigma-Aldrich) dissolved in 0.7% sodium chloride, and administered i.p. at 20 μl/g of body weight, according to two procedures: (1) pulse administration: a single injection followed by post-thymidine analog survivals of 1 (N = 3), 7 (N = 2), or 30 days (N = 3); and (2) sequential administration: four daily injections followed by survivals of 90 (N = 2) or 180 days (N = 1).
In vivo Neuronal Tracer Administration
To reveal the differentiation of cerebellar newborn cells into the neuronal phenotype, Neurobiotin tracer (Vector Laboratories, Inc., Burlingame, CA, USA) was applied in vivo at the molecular layer of the Cb, 86 or 176 days after repetitive CldU administration. Animals were anesthetized and the soft tissue over the rostralmost portion of the sagittal suture was carefully removed with the tip of a scalpel (Supplementary Figure 3A). Then, a small perpendicular and superficial incision was made in order to disrupt this portion of the sagittal suture and expose the dorsal surface of the rostral portion of CCb. After slightly cutting the cerebellar surface, crystals of Neurobiotin were applied with the tip of a needle (Supplementary Figure 3B). Finally, the wound was sealed with Histoacryl® (B. Braun Aesculap AG, Tuttligen, Germany), animals were allowed to recover from anesthesia and returned to their tanks.
Double Immunohistochemistry (CldU Label Retention and Neuronal Markers' Expression)
To break double-stranded DNA into single strands and expose the proliferation marker CldU to the antibodies, free floating tissue sections were first incubated in 2 N HCl (Baker, Phillipsburg, N.J. USA) in PB containing 0.3% Triton X-100 (Baker; PB-T) for 50 min at room temperature, followed by rinsing in PB (3 × 10 min). Then, sections were incubated for 1–2 days at 4°C in rat anti BrdU-CldU antibody (Accurate Chemical & Scientific Corporation, Westbury, NY, USA) at a dilution of 1:500 in PB-T, along with other primary antibody [rabbit anti doublecortin (Abcam, Cambridge, MA, USA) at 1/2,000 dilution, mouse anti HuC/HuD (Molecular Probes, Eugene, OR, USA) at 1:200 dilution, or rabbit anti TH (ThermoScientific, Waltham, MA USA) at 1/800 dilution]. Sections were rinsed in PB (3 × 10 min) and incubated in a mixture of donkey anti rat Cy5 secondary antibody (Jackson Immuno Research, West Grove, PA, USA) at 1:1,000 dilution and goat anti mouse Alexa 488 (Jackson Immuno Research) at 1:1,000 dilution in PB-T, for 90 min at room temperature. After rinsing in PB (3 × 10 min), sections were mounted in PVA/DABCO cover slipping solution. Negative controls involved the omission of CldU or of primary antibodies incubation; both controls resulted in no detectable staining (data not shown).
Simultaneous Demonstration of CldU Label Retention and Neuronal Tracer Labeling
In order to evidence the co-localization of CldU and Neurobiotin, sections were first pretreated in HCl and incubated in rat anti BrdU-CldU as described above. After rinsing in PB (3 × 10 min), sections were incubated during 90 min in donkey anti rat Cy5 at 1:1,000 dilution, together with streptavidin Cy3 (VECTOR) at a 1:500 dilution in PB-T. Sections were finally rinsed in PB (3 × 10 min) and mounted in PVA-DABCO coverslipping solution for immunofluorescence.
Image Acquisition and Processing
Most sections were imaged on a confocal system consisting of an Olympus BX61 microscope equipped with a FV300 confocal module and four lasers lines (405, 488, 543, and 633 nm) and the following objectives: 4x: UPlanFLN 0,13AN, 10x: UplanSAPO 0,40AN, 20x: UPlanFI 0,50AN, 40x: UPlanFI 0.75AN, and 60x: Plan ApoN 1,42AN objectives of the Confocal Microscopy Facility (IIBCE). Others were imaged on a Leica TCS SP5 II microscope equipped with four lasers lines (405, argon multiline 458, 476, 488, and 514 nm, and HeNe 543 and 633 nm), and HC PL FLUOTAR 5x/0.15, HC PL APO 20x/0.70 CS, HCX PL APO 40x/1.25-0.75 Oil, HCX PL APO 63x/1.40-0.60 Oil, HCX PL APO 63x/1.20 W CORR, and PL APO 100x/1.40-0.70 Oil CS objectives of the Confocal Microscopy Unit (Facultad de Medicina, UdelaR).
Acquisition settings were adjusted to ensure the completely dynamic range detection. Images of confocal planes were sequentially scanned with each laser line. Fifteen confocal planes, every 2 μm, were acquired in sections of levels L1–L3. For levels L4–L6, 15, 20, 25 to 30 confocal planes, every 0.5 or 1 μm were acquired. Post-processing of images was limited to small changes in the distribution histogram or background subtraction (Fiji Rolling ball radius: 50 pixels) in most cases.
Co-expression of markers was confirmed by orthogonal projections in the X-Z and Y-Z planes of the z-stacks at X-Y position of presumptive co-localization and/or visualization of the images corresponding to each channel of a single plane separately along with their overlay.
We used the same nomenclature and abbreviations as previously (Maler et al., 1991; Zupanc et al., 1996; Corrêa et al., 1998; Meek and Nieuwenhuys, 1998; Olivera-Pasilio et al., 2014).
To quantify the amount of labeled cells per section in levels L1–L3, we constructed 3-D models of the sections from serial 2D low power confocal microphotographs with BioVis3D (R) as detailed in Iribarne and Castelló (2014). The boundaries of the olfactory bulb (OB), and internal cell layer were drawn and the location of every labeled nucleus was indicated in each plane of the 3D reconstruction with the tool “dot sets.” The spatial distribution of labeled nuclei was evidenced by making transparent the constructed models.
We also used BioVis3D to determine the location of labeled nuclei in the x and y axes. First, we established the crossing of the mid-line and dorsal border of the OB as the origin of the x and y axes (red lines in Supplementary Figure 1). Then, lines extending from each nucleus to the x and y axes (green and blue lines in Supplementary Figure 1) were drawn and their length was calculated by the software. The resulting values were normalized by the width and height of each region of interest at each studied level to calculate the relative distance of every nucleus.
For every level (L1–L3) of each chase duration (1, 7, and 30 days), the mean and standard deviation of the total amount of labeled nuclei per section were calculated. We also quantified the amount of labeled nuclei within and outside the internal cell layer of L1 and L2 (Supplementary Figures 4A,B), and within and outside the ventricular proliferation zone adjacent to the ventral and dorsal subdivisions of the ventral telencephalon of L3 (Supplementary Figure 4C).
Differentiation into the neuronal phenotype by demonstration of the expression of neuronal markers (HuC/HuD or TH) or retrograde Neurobiotin labeling of long term CldU label retaining newborn cells was quantified with the aid of Fiji-ImageJ Point tool. In z stacks of the brain regions of interest, CldU+ nuclei, and double labeled CldU+/HuC/HuD+, CldU+/TH+, or CldU/Neurobiotin cells were marked in selected equally spaced confocal planes to avoid over counting. The total amount of each class was registered and the percentages of CldU+ cells that expressed neuronal markers or were labeled with Neurobiotin were calculated.
We analyzed variations in the amount of CldU labeled cells per section using One-way ANOVA or Mann-Whitney U-test, after determining the variance of the samples with Kolmogorov-Smirnov test. Differences among groups were considered significant when p < 0.05.
Spatial Distribution of Brain Proliferation Zones
We first analyzed the spatial distribution of brain proliferation zones in adult G. omarorum as a reference to depict the migration and/or differentiation of newborn cells. The spatial distribution of CldU labeled cells after a short survival (1 day) following the administration of a pulse of CldU (red dots in Figure 1) reproduced previous findings (Olivera-Pasilio et al., 2014). Briefly, most proliferating cells populated ventricular proliferation zones at the lining of the telencephalic (L2, L3, Figure 1), mesencephalic, diencephalic (L4, L5, Figure 1), and rhombencephalic (L6, Figure 1) ventricles. Outstanding: clusters of proliferating cells were found in all cerebellar divisions (L4, L5, Figure 1) and in the lateral-caudal pole of the ELL (L6, Figure 1). This spatial pattern allowed us to depict the boundaries of proliferation zones that were used as a reference to determine whether derived cells persist within the proliferation zones or migrate toward other regions or sub-regions at longer survival times (7–180 days).
Migration of Newborn Cells
Some labeled cells remained within the proliferation zones after post CldU survival times between 7 and 180 days. Conversely, most of the CldU labeled cells were located at increasingly greater distances from the proliferation zones boundaries, according to the survival duration. This shift is exemplified in Figure 1 for survivals of 1 and 30 days (red and blue dots in Figure 1). The abundance of migrating newborn cells and the locations that they reached as a result of the migration varied among proliferation zones. In this work we focused on the brain regions where the migration process was more salient: the rostral telencephalon and OB, the TeO, the TS, and the Cb.
Olfactory Bulb and Rostral Telencephalon
The sessile OB of G. omarorum shares the histoarchitecture of teleost's OB (Byrd and Brunjes, 1995; Kermen et al., 2013), consisting of a round core of small and densely packed cells, the internal cell layer (ICL) surrounded by three concentric diffuse layers: the external cell layer (ECL), the glomerular layer (GL), and the outer primary olfactory fiber layer (POFL) adjacent to the OB's surface (L1 and L2 in Supplementary Figure 1).
One day after a pulse of CldU, labeled cells were rare in the OB. Few and scattered proliferating cells were located at any of the layers of the rostral and medial part of the OB (red dots in L1 and L2, Figure 1: double arrows in AL1 and AL2, Figure 2; red dots in AL1 and AL2, Figure 3A). Conversely, densely packed CldU labeled cells were found at the lining of the most rostral portion of the telencephalic ventricle, nearby the caudal OB and the rostral region of the ventral (Vv) and dorsal (Vd) subdivisions of the subpallium. There, proliferating cells formed an extended ventricular proliferation zone (zone 1b, Olivera-Pasilio et al., 2014; red dots lining the ventricle at the zones indicated by the green rectangles in L2 and L3, Figures 1, 3A; arrows in AL2 and AL3, Figure 2). This rostral-caudal gradient in the amount of proliferating cells was confirmed quantitatively as the number of proliferating cells in the rostral and caudal part of the OB was significantly lower than in the rostral portion of the subpallium 1 day after CldU administration (Figure 3B).
Figure 2. Spatial-temporal distribution of proliferating cells and derived cells in the rostral (L1) and caudal (L2) regions of the OB, and rostral subpallium (L3) in G. omarorum. Images correspond to microphotographs of frontal sections of the brains of animals treated with a single (A–C) or four daily doses (D,E) of CldU followed by 1 (A), 7 (B), 30 (C), 90 (D), and 180 (E) days of survival. The OB is almost devoid of CldU+ cells after short survivals (A L1, L2). Conversely, the lining of the rostral portion of the telencephalic ventricle, adjacent to the subpallium was populated by densely packed CldU labeled cells, conforming a clear proliferation zone (arrows in A L2, L3). From 1 to 30 days CldU+ cells appeared within the nerve tissue at progressively greater distances from the proliferation zones at L2 and L3. At longer chases (90 and 180 days), CldU+ cells also populate the rostral OB, and appeared to increase in number in L1–L3. ECL, External cell layer; Er, Rostral entopeduncular nucleus; FB, Forebrain bundle; GL, granular layer; ICL, Internal cell layer; MOTF, medial olfactory terminal field; POFL, V, Ventricle; Vc, Ventral telencephalon, central subdivision Vl, Ventral telencephalon, lateral subdivision. Scale bars: 100 μm.
Figure 3. Spatial-temporal distribution and quantification of proliferating and derived cells within the rostral telencephalon. (A) The location of proliferating cells is represented by red dots in the 3D reconstructions of rostral (L1) and caudal (L2) olfactory bulb and rostral subpallium (L3). Proliferation zones were located at the ventricular lining indicated by green rectangles in L2 and L3. (B) Bar plots of the amount of labeled cells per section at the three levels studied (L1–L3) following 1 (N = 3), 7 (N = 2), and 30 (N = 3) days after the administration of a pulse of CldU. Values are expressed as the mean and standard deviation of the total amount of labeled cells per section. * <0.05, One-way ANOVA.
Seven days after CldU administration, proliferating cells were also located predominantly at ventricular proliferation zones in the caudal portion of the OB and rostral subpallium (BL1–L3, Figure 2). Only few CldU labeled nuclei were placed throughout the OB layers or the subpallium. The number of labeled cells increased in all levels at this chase duration, but only significantly at L3. The rostral-caudal gradient was preserved but steeper (Figure 3B).
Thirty days after CldU administration, some proliferating cells remained within the boundaries of the proliferation zone 1b adjacent to the caudal OB (CL2, Figure 2) and rostral subpallium (CL3, Figure 2). Unlike shorter chases, some CldU labeled nuclei were located at considerable distances from the rostral region of the proliferation zone 1b, reaching the ICL of caudal and, in a less extent, rostral OB (CL2 and CL1, Figure 2). The amount of CldU labeled cells in L1 and L2 increased up to 2.4 and 3.7 times the values found 1 day after CldU administration, respectively. However, only L1 showed significant differences in the amount of CldU labeled cells between both chases. Conversely, the amount of CldU labeled cells decreased significantly in L3 from 7 to 30 days (Figure 3B). Few CldU labeled nuclei were found lateral to the caudal zone of 1b (adjacent to the subpallium), reaching Vd, Vv, MOTF, and medial zone of FB (CL3, Figure 2).
CldU label retaining cells spilled out the boundaries of the ICL of the caudal OB at a 90 day chase (Figure 2, EL2) whereas most labeled cells remain within the ICL boundaries of the ICL of the rostral OB (Figure 2, EL1). At 180 day chase the spilled out of labeled cells from the ICL of the rostral OB to the surrounding layer was evident (Figure 2, FL1).
The amount of CldU label retaining cells in the lateral zone of the subpallium increased considerably 90 and 180 day after CldU administration. At 90 days newborn cells predominate in the ventral zone, whereas at 180 days were distributed along all the dorso-ventral extension of the subpallium.
All the divisions of the Cb of G. omarorum (CCb, valvula cerebelli -VCb, and caudal lobe, including the eminentia granularis anterior -EGa- and posterior -EGp-), are organized in three layers, molecular, ganglionic, and granular, as exemplified in Supplementary Figure 5A. The ganglionic layer consists of Purkinje and eurydendroid cells. Eurydendroid cells, which are the origin of Cb efferents, are not aggregated in nuclei unlike other vertebrates (Finger, 1978).
Remarkable migrations processes both for the abundance of migrating cells as well as for their final destination, were detected in all cerebellar divisions as previously described (Olivera-Pasilio et al., 2014). Proliferation zones were circumscribed to a single cerebellar layer or even a region within a single cerebellar layer (red dots in L4 and L5, Figure 1).
The proliferation zone of the CCb, evidenced by the distribution of proliferating cells at 1 day chase, occupied the medial zone of its molecular layer (CCb-mol; red dots in L4, Figure 1). Thirty days after CldU administration, derived cells were mainly found at the granular layer of CCb (CCb-gra; blue dots in L4, Figure 1). However, scarce and intensely labeled CldU cells remained within the proliferation zone's boundaries.
In the VCb a conspicuous proliferation zone occupied all the extension of the molecular layer (VCb-mol). Proliferating cells were more densely packed near the dorsal-medial region of VCb-mol and migrating cells were sparsely and homogeneously found in all the extension of the granular layer (VCb-gra).
The proliferation zone of the caudal lobe of the Cb occupied the granular layer of the medial granular eminence (EGm-gra) while derived cells were located at the granular layer of the posterior granular eminence (EGp-gra) as shown in Olivera-Pasilio et al. (2014).
The TeO is a multimodal integration center which is interconnected with the torus longitudinalis forming a Cb-like structure (Bell, 2002). In G. omarorum, it is a hollow hemispheric shaped structure. It has a cortical histoarchitecture and consists of seven cellular and fibrillary alternating layers (Supplementary Figure 5B; Meek and Nieuwenhuys, 1998). Proliferating cells were located at the dorsal-medial and ventral-lateral border of the caudal pole of TeO, forming a horseshoe shaped ribbon-like proliferation zone. One day after CldU administration, proliferating cells were distributed in all TeO layers (red dots in L4 and L5, Figure 1), though appeared to be more densely packed in deeper layers as the stratum periventriculare (SPV). At longer chases, CldU label cells occupied more superficial layers of TeO, also extending beyond the proliferation zones' boundaries in the rostral direction (blue dots in L4 and L5, Figure 1).
One hundred eighty days after CldU administration, derived cells were located ~100 μm away from the dorsal region of the proliferation zone at rostral levels of the caudal TeO. These long labeled retaining cells were grouped mainly at the SPV and SAC layers, and less frequently reached the SGC (L5, Figure 1).
The TS of G. omarorum is a spherical protrusion of the mesencephalic tegmentum beneath the TeO. It is a layered structure which receives octavolateral inputs from rhombencephalic primary brain centers (Meek and Nieuwenhuys, 1998). One day after CldU administration proliferating cells were located at the medial and lateral borders of the caudal pole of TS (red dots in L5, Figure 1), forming a ring-shaped proliferation zone. At longer chases derived cells appeared diffusely distributed at the caudal pole of TS (blue dots in L5, Figure 1).
Electrosensory Lateral Line Lobe
The ELL is the primary relay nucleus of electrosensory pathways. It is a layered cerebellum-like structure (Supplementary Figure 5C; Meek and Nieuwenhuys, 1998) in which principal cells project to contralateral rhombencephalic and mesencephalic structures (praeminentialis nucleus and TS) which project back to the ELL, either directly or indirectly through Cb. At 1 day chase duration, proliferating cells were mainly located at the lateral-caudal border of cellular layers of ELL, and showed a medial-lateral and rostral-caudal gradient (red dots in L6, Figure 1). At longer chases, ELL CldU label retaining cells were extensively and diffusely distributed (blue dots in L6, Figure 1).
Neuronal Differentiation and Insertion into Neuronal Circuits
With the aim of studying neuronal differentiation and neurogenic capacity of G. omarorum adult brain proliferation zones, we analyzed the expression of neuronal markers, including the early neuronal markers DCX, and HuC/HuD or markers of further differentiation into the neuronal phenotype as tyrosine hydroxylase (TH), in CldU label retaining cells after post thymidine analog administration chases ranging from 7 to 180 days. We also assessed the insertion of newborn neurons into pre-existing neural circuits of the CCb by “in vivo” retrograde labeling of granule cell after Neurobiotin administration at the molecular layer of CCb.
Neuronal Differentiation in the Olfactory Bulb and Rostral Telencephalon Evidenced by Co-localization of CldU and HuC/HuD, DCX, or TH
One day after thymidine analog administration, DCX labeled a net of processes beneath the ventricular proliferation zone adjacent to the medial and dorsal-medial zone of the telencephalic proliferation zone 1b (inset, Supplementary Figure 6A). We only found CldU-DCX double labeled cells adjacent to the ventral region of this proliferation zone (Supplementary Figure 6B) as evidenced by the overlay of CldU and DCX signals corresponding to a single confocal plane (Supplementary Figure 6C) or by orthogonal projections of a z stack (Supplementary Figure 6D). At this chase duration, we did not find CldU-DCX or CldU-HuC/HuD double labeled cells in any other brain region.
Seven days after CldU administration, some cells at the ventral part of the subventricular zone of the rostral subpallium were CldU-HuC/HuD double labeled (Figure 4), but not at the rostral or caudal zones of the OB. Unexpectedly, we did not find any CldU-DCX double labeled cell at this chase duration.
Figure 4. Neuronal differentiation in the subpallium at 7 days after the administration of a pulse of CldU demonstrated by co-localization with HuC/HuD. (A) Confocal microphotographs of the ventricular lining at the region of the rostral subpallium indicated by the rectangle in the panoramic view (inset). HuC/HuD and CldU labeling are shown in green and red channels in the microphotographs of a single plane shown in (A,B), respectively. The overlay of both channels is shown in (C). Arrowheads indicate CldU labeled retaining cells also expressing the neuronal marker HuC/HuD. Scale bars: (inset) 100 μm; (A–C) 20 μm.
After a 30 day chase, CldU label retaining cells expressed HuC/HuD at the ICL of the caudal OB (Figure 5A) and the ventral region of the subventricular zone of the rostral subpallium (Figure 5B). CldU-HuC/HuD double labeled cells' nuclei were round and the chromatin either densely (Figure 5A) or loosely (Figure 5B) packed. Some newborn CldU labeled cells with fusiform shape and elongated nuclei with densely packed chromatin also express DCX (Figures 5C,D).
Figure 5. Neuronal differentiation in the olfactory bulb and rostral subpallium at 30 days after the administration of a pulse of CldU demonstrated by co-localization with HuC/HuD and DXC. (A,B) Confocal microphotographs of the caudal OB and rostral subpallium at the regions containing double labeled cells indicated by the dotted squares in the panoramic views (insets), respectively. HuC/HuD and CldU labeling are shown in green (left) and red (middle) channels; the right image corresponds to the overlays of both channels. (C,D) x-z and y-z orthogonal projection of stacks of 35 confocal planes scanned every 0.5 μm at the lines crossing at the cell of interest, confirming the co-localization of CldU and DCX in the rostral subpallium at the positions indicated by the dotted rectangles in the panoramic views (insets). Scale bars: (A,B) 10 μm; (C,D) 5 μm; insets, 100 μm.
Double labeled CldU-HuC/HuD cells were found at the ICL (Figure 6A) and the dorso-medial zone (Figure 6B) of the rostral OB 90 days after CldU administration. All CldU-HuC/HuD double-labeled cells had ovoid to round nuclei surrounded by a thin cytoplasm without evident cellular processes. At 90 days CldU-HuC/HuD double-labeled were also found at L3 (Figure 6C).
Figure 6. Neuronal differentiation in the olfactory bulb and rostral subpallium at 90 days after four daily injections of CldU demonstrated by co-localization with HuC/HuD. Confocal microphotographs of the olfactory bulb (A,B,B′) and the rostral subpallium (C,C′) at the level indicated by the dotted rectangles in the panoramic view (insets) to evidence double labeled cells. HuC/HuD and CldU labeling are shown in green and red channels of single scans, respectively. Co-localization is confirmed by the overlay of both channels, or by the x-z and y-z orthogonal projections of stacks obtained from 19 planes, every 0.5 μm (B′), or 15 planes, every 0.5 μm (C′).
At 90 days, double labeled CldU-DCX cells were only found at the dorsal-medial zone of the rostral level of OB (data not shown).
At this chase duration CldU labeled cells also express TH at the ventricular or sub ventricular zone of the rostral subpallium (Figure 7). Some of these cells showed a thin cytoplasmic halo without cellular processes (Figures 7A,A′) whereas others had more expanded cytoplasm from which thin and short cellular processes with few branching points emerge (Figure 7B, arrowheads in Figure 7B′).
Figure 7. Neuronal differentiation in the rostral subpallium at 90 days after after four daily injections of CldU demonstrated by co-localization with TH. (A,B) Confocal microphotographs of the subpallium at the regions indicated by the dotted rectangles in the panoramic views (insets). Co-localization is demonstrated by TH and CldU labeling of a single confocal plane and the overlay of both images (A,B). Co-localization is also confirmed by the x-z and y-z orthogonal projections of 16 confocal planes, every 0.5 μm (A′) or 45 confocal planes, every 0.5 μm (B′). Arrows indicate neuronal processes of a newborn neuron. Scale bars: (A,B) 20 μm; (A′,B′) 5 μm; insets 100 μm.
One hundred eighty days after CldU administration, double labeled CldU-TH cells were found in the rostral subpallium, far from the proliferation zone (Figure 8), and at both, caudal (Figure 9) and rostral (Figure 10) levels of the OB. Some newborn cells had an ovoid nucleus surrounded by a thin cytoplasmic halo without cellular processes, as those found lateral to the subpallial proliferation zone (Figures 8B,C). Many double labeled cells showed a larger cytoplasmic halo from which two or three relatively thick cellular processes emerged from opposite regions of the cell body. These cells resembling bipolar or multipolar neurons were located at the ICL of caudal (Figures 9B,B′,C,C′, Supplementary Video 1) and rostral (Figures 10C,C′,C″) OB. In other cells at the ICL of the rostral OB, a relatively large nucleus occupied an asymmetric location respect to a very thin cytoplasmic halo, resembling migrating neuroblasts (Figures 10A,B). All double labeled CldU-TH cells were intermingled with cells with single labeled CldU+ nuclei or TH+ cytoplasm.
Figure 8. Neuronal differentiation in the rostral subpallium at 180 days after four daily injections of CldU demonstrated by co-localization with TH. (A) Maximal intensity projection of 15 confocal planes taken every 2 μm at the rostral subpallium. (B) x-z and y-z orthogonal projection of 25 confocal planes, every 2 μm, confirming the co-localization of CldU and TH in a cell at the region indicated by the dotted rectangle in (A). (C) Co-localization of TH and CldU is also confirmed by the overlay of the sequentially acquired channels a single plane. Scale bars (A) 100 μm; (B,C) 5 μm.
Figure 9. Neuronal differentiation in the caudal olfactory bulb at 180 days after four daily injections of CldU demonstrated by colocalization with TH. (A) Topographic confocal image of a frontal section of the caudal olfactory bulb. The rectangles indicate the locations at which higher power confocal images were acquired (B,B′,C,C′). Images corresponding to both channels of a single confocal plane and the overlay at the regions indicated by the dotted rectangles in (A) are shown in (B,C′). (B') x-z and y-z orthogonal projection of 22 confocal planes, every 1 μm, confirming the colocalization of CldU and TH in the same cell as in (B). Scale bars: (A) 50 μm; (B–C') 5 μm.
Figure 10. Neuronal differentiation in the rostral olfactory bulb at 180 days after four daily injections of CldU demonstrated by co-localization with TH. Microphotograph at the region of the rostral OB indicated by the rectangle in the inset in (A). (B) Higher power images of both channels and the overlay of the region containing a cell of interest at the region indicated by the dotted square in the inset in (A). (C) Maximal intensity projection of a stack of 17 confocal planes, every 0.5 μm. The rectangle indicates the location of a cell which co-localization was demonstrated by x-z and y-z orthogonal projections of the same stack (C′) as well as each channel and overlay of the sequentially acquired channels a single plane (C′′). Scale bars: (A) 20 μm; (B, Inset in A) 100 μm; (B,C′′) 5 μm.
According to the quantitative analysis, almost 0.5% of long term CldU retaining new born cells at the lateral regions of the subpallium (L3) expressed the mature neuronal marker TH+ after a 180 day chase. The fraction of CldU labeled cells that also expressed TH reached almost 1% and more than 1.5% of the total amount of CldU labeled cells at the caudal (L2) rostral (L1; Table 1).
Neuronal Differentiation in the Corpus Cerebelli and Cerebellum-Like Structures Evidenced by Co-localization of CldU and HuC/HuD
After a short thymidine analog survival (7 days), we did not find HuC/HuD expression in CldU labeled cells. However, longer survivals (30, 90, and 180 days) allowed us to evidence the differentiation of derived cells into neurons in the CCb and other Cb-like structures.
We did not find CldU-DCX double labeled cells in CCb-mol 1 or 7 days after CldU administration, even though DCX processes were abundant at the CCb-mol (running parallel to the cerebellar surface in the medial-lateral direction) and the Purkinje cells' layer (running parallel to the cerebellar surface in the rostral-caudal direction; Supplementary Figure 7).
Thirty days after CldU administration, scarce CldU labeled cells at the CCb-gra also expressed HuC/HuD (Figure 11A). These double labeled cells were small, with an ovoid or polygonal nucleus and granular CldU labeling of varied intensity, surrounded by a thin polygonal cytoplasmic halo (Figure 11B). Double labeled cells were intermingled with a myriad of HuC/HuD+ cells of the CCb-gra.
Figure 11. Neuronal differentiation in the corpus cerebelli at 30, 90, and, 180 days after four daily injections of CldU demonstrated by co-localization with HuC/HuD. (A) Low power microphotograph at the region of the corpus cerebelli. The dotted rectangle indicates location of a double labeled cell, as illustrated by the microphotographs of each channel and the overlay (B) in the inset in (A). (C) Higher power image of a stack of 25 confocal planes, every 0.5 μm. The rectangle indicates the location of a cell which co-localization was demonstrated by the x-z and y-z orthogonal projections of the same stack (C') as well as each channel and overlay of a single plane (C″). Scale bars: (A) 20 μm; (B, Inset in A) 100 μm; (B,C”) 5 μm.
Double-labeled CldU-HuC/HuD cells with similar labeling characteristics were found at the CCb-gra 90 (Figures 11C,C′) and 180 days (data not shown) after CldU administration.
Purkinje and/or eurydendroid cells show a marked expression of HuC/HuD but did not showed co-localization with CldU at any of the chases studied.
Tectum opticum and torus semicircularis
Similar to the CCb, we did not find double labeled CldU-DCX newborn cells in the TeO at any of the chases studied, even though bundles of DCX processes were abundant beneath the dorsal-medial tectal proliferation zone (Supplementary Figure 8).
Ninety days after CldU administration, long term label retaining cells also expressed HuC/HuD at the deeper layers of the caudal pole of the TeO (Figure 12). Double labeled cells were found in all dorsal-ventral extension of the stratum periventriculare (SPV), and in lesser density at the boundaries between stratum album centrale (SAC) and stratum griseum centrale (SGC). Most double labeled cells had round to ovoid nucleus surrounded by a thick cytoplasmic halo without cellular processes (Figures 12A–D). Likewise, CldU label retaining cells also expressing HuC/HuD with round morphology were found at the ventral region of the TS. Double labeled cells showed a round morphology (Figures 12E,F).
Figure 12. Neuronal differentiation in the tectum opticum and torus semicircularis at 90 and 180 days after four daily injections of CldU demonstrated by co-localization with HuC/HuD. (A) Maximal intensity projections of confocal microphotographs of a z stack (20 μm, every 0.5 μm) at the caudal pole of the tectum opticum (TeO) and torus semicircularis (TS). The dotted rectangles indicate location of two regions of interest observed at higher magnification in (B,E). Double labeling of tectal cells (B,C,C′,D) was confirmed by the microphotograph of each channel and of the overlay (C) as well as the x-z and y-z projection of two stacks (C′,D). Double labeling of toral cells is demonstrated in (F) by microphotographs of each channel and of the overlay of the region indicated by the dotted rectangle in (E). Scale bars: (A,B,E) 50 μm; (C,C′,D,F) 5 μm.
One hundred eighty days after CldU administration, derived cells were mainly grouped at the SPV and SAC layers at about 100 μm from the rostral portion of the dorsal-medial region of the TeO proliferation zone (asterisk in Figure 13A). Some of these cells expressed HuC/HuD (arrows in Figures 13A–C). Conversely, most of CldU labeled were not displaced from the ventro-lateral region of the tectal proliferation zone (arrow in Figure 13D); few others were located quite far from it (double arrows in Figures 13D,E). Some of these long term CldU label retaining cells also expressed HuC/HuD (Figure 13E).
Figure 13. Neuronal differentiation in the intermediate region of the optic tectum and torus semicircularis at 90 and 180 days after four daily injections of CldU demonstrated by co-localization with HuC/HuD. (A,B) Low power microphotographs at the dorsal-medial and ventral-lateral border of the tectum opticum (TeO) and dorsal region of the torus semicircularis (TS), rostral to the caudal pole. The dotted rectangles indicate the location of three regions of interest observed at higher magnification in (B,E,F), respectively. Double labeling of tectal cells (B,C,E) and toral newborn cells (F,G) was confirmed by the overlay of each channel (C) and xy and zy orthogonal projections a stacks. Scale bars: (A,B,D,F) 20 μm; (B, Inset in A and D) 100 μm; (C,E,G) 5 μm.
In the ventral region of the TS, long term CldU labeled cells were distributed in and extended zone with numerous double CldU-HuC/HuD labeled cells (Figures 13D,F,G).
Electrosensory lateral line lobe
Unlike other brain regions, very scarce CldU long-term label retaining cells were found at the caudal region of the ELL 90 (Figures 14A,B) or 180 (Figure 14C) days after CldU administration. Some of these cells with a thin fusiform to ovoid cytoplasmic halo were located at the GCL, near the boundaries with adjacent layers, also expressing HuC/HuD (Figures 14 A′,A′′,B′,C′,C′′).
Figure 14. Neuronal differentiation in the caudal pole of the electrosensory lateral line lobe at 90 and 180 days after four daily injections of CldU demonstrated by co-localization with HuC/HuD. (A–C) Low power microphotographs of frontal sections at the lateral-caudal border of the electrosensory lateral line lobe. The dotted rectangles indicate the location of double labeled CldU-HuC/HuD newborn cells as evidenced by the overlays of sequentially acquired images (A′–C′) and orthogonal projections of stacks (A′′,C′′). DNL, deep neuropile layer of ELL; DFL, deep fiber layer of ELL; GCL, granular cell layer of ELL; PCL, pyramidal cell layer of ELL; mol, molecular layer of ELL. Scale bars: (A–C) 50 μm; (A′,A′′,B′,C′,C′′) 5 μm.
Considering the quantitative data from all the analyzed brain regions (OB, TeO, TS and CCb), 50% of long term CldU retaining new born cells expressed HuC/HuD 90 days after CldU administration (range: TS: 33,33—CCb: 57,14). The fraction of double labeled cells increased up to almost 80% in the TS and TeO after 180 day chase (Table 1).
Neuronal Differentiation in the CCb Evidenced by CldU and Neurobiotin
Repetitive CldU administration allowed the long term retention of CldU in numerous cells at the CCb-gra, both 90 (Figure 15A) and 180 days (Figure 15B) after thymidine analog administration. These derived cells probably correspond to granule cells, both because of their location, as well as the shape and size of their nuclei. Cortical application of Neurobiotin labeled many cells with small round, ovoid, or polygonal soma, at the CCb-gra at both chase durations, even far from the site of tracer application. Note that the site of injection is not visible in the topographic images of Figures 15A,B, and thus is located more than 200 μm from the soma of the Neurobiotin labeled cells. This indicates that the tracer was incorporated into the axons or end terminals of the labeled cells at the CCb-mol and retrogradely transported up to the cell's soma and perisomatic dendrites at the CCb-gra. This, as well as the known histoarchitectural organization of the Cb, further supports the identification of these cells as granule cells. Many long term CldU retaining cells were labeled with Neurobiotin (Figures 15A′,B′,B″, Supplementary Video 2), indicating that the newborn cells acquired the mature granular morphology in 90 days. Also indicates that these newborn granule cells very probably were incorporated into the local cerebellar circuit and might be already functional. Conversely, Purkinje cells were also labeled with Neurobiotin but not CldU.
Figure 15. Neuronal differentiation in the corpus cerebelli at 90 and 180 days after four daily injections of CldU demonstrated by co-localization retrogradely transported Neurobiotin. (A,B) Low power microphotograph of frontal sections at the corpus cerebelli (CCb). The dotted rectangles indicate the location of double labeled newborn cells nearby the boundary between molecular (CCb-mol) and granular (CCb-gra) layer of the CCb (A), or within CCb-gra (B). The double labeling was confirmed at higher magnification by the microphotographs of each channel and the overlays (A′,B′,B′′) as well as by the 3-D visualization as shown in the Supplementary Video 2. Scale bars: (A) = 20 μm; (B, Inset in A) = 100 μm; (A′,B′,B′′) = 5 μm.
The fraction of CldU CCb-gra labeled cells that were retrogradely labeled represented almost 1% and more than 9% after chase durations of 90 and 180 days, respectively (Table 1).
Adult neurogenesis, whether involved in protracted postnatal development of parts of the brain, the persistent addition of new neurons (constitutive neurogenesis), cellular turnover, or the regeneration after injury (Grandel and Brand, 2013) is a widespread process in the animal kingdom, from the most primitive species in which the nervous system first evolved to diverse vertebrate radiations.
Though adult cell proliferation was studied in teleost (Rahmann, 1968) soon after the discovery of adult neurogenesis in mammals by Altman (1962), only few species of the numerous teleostean radiation have been studied. Even fewer are the teleost species in which adult neurogenesis was demonstrated. Remarkably, proliferating cells give place to newborn neurons in a period as short as 24 h after BrdU administration in several brain regions (OB, TEL, TO, TL, and Cb) of Austrolebias (Fernández et al., 2011; Rosillo et al., 2016), probably related to the short duration of their life cycle. In all other studied teleost species, longer chases are necessary for the demonstration of neurogenesis: 3 days in the dorsal telencephalon of D. rerio (Adolf et al., 2006), 7 days in the TEL, TeO, and Cb of N. furzeri (Terzibasi et al., 2012), 15 days in the OB and TEL of D. rerio (Adolf et al., 2006). Almost 50% of the total amount of proliferating cells differentiates into neurons at 270–744 days chases in D. rerio (Zupanc et al., 2005; Hinsch and Zupanc, 2007) though a great variation among brain regions exists. A high and variable proportion of adult brain cells expressing HuC/HuD in O. mossambicus was demonstrated 100 days after BrdU administration (Teles et al., 2012).
G. omarorum brain develops rostro-caudally; as morphogenesis develops, the widespread distribution of larval brain proliferating cells is progressively reduced but persist in several ventricular and extraventricular proliferation zones up to adulthood (Iribarne and Castelló, 2014; Olivera-Pasilio et al., 2014). In the present work we deepened the study of the migration process (particularly at the rostral telencephalon and OB), and demonstrate the differentiation into the neuronal phenotype of newborn cells generated in telencephalic, mesencephalic, and rhombencephalic proliferation zones.
Adult G. omarorum Brain Proliferation Zones are the Source of Long-Range Migratory Streams
According to the chase and the brain region, newborn cells were found close to the proliferation zones from where they originate or at increasing distances from their boundaries. At 7–180 days survivals after CldU administration we evidenced wide-ranging migrating cells with thin and elongated nuclei (usually intensely stained with CldU) surrounded by thin elongated cellular process of diverse lengths, typical characteristics of migrating neuroblasts. Other cells had round to ovoid nuclei, with granular or diffuse CldU staining, indicative of cells that already reached their final location.
No proliferation zone was found at the rostral region of G. omarorum OB. Despite that, the OB was progressively populated by CldU labeled cells at chase durations from 7 to 180 days.
Considering that the nearest proliferation zone was found at the ventricular lining of the rostralmost region of the telencephalic ventricle (adjacent to the caudal portion of OB and the rostral portion of the subpallium), we inferred that this is the main source of OB newborn cells. Taking into account the location of CldU labeled nuclei at the three telencephalic levels studied as a function of chase duration, we propose a three-step migration process. First, a medial-lateral migration from the proliferation 1b to adjacent regions of the subpallium and caudal OB; second, a caudal-rostral migration along the ICL and the dorsal-medial zone of the caudal and rostral OB; finally, a radial migration to populate other layers of caudal and rostral levels of OB. This resembles the rostral migratory stream from the telencephalic ventricle to the OB described in mammals.
Even though the rostral migratory stream was first demonstrated in mammals (Altman, 1969), a similar mechanism of cell proliferation at the wall of the telencephalic ventricle and collective cellular migration was also demonstrated in birds (Goldman and Nottebohm, 1983; Nottebohm, 2002; Barnea and Pravosudov, 2011), and only recently identified in D. rerio (Adolf et al., 2006; Grandel et al., 2006; Pellegrini et al., 2007), and supported by ex vivo imaging by Kishimoto et al. (2011). The generality of this process among teleost was suggested by Olivera-Pasilio et al. (2014) and supported by Lasserre (2014) in the phylogenetically close teleost G. omarorum and by Rosillo et al. (2016) in Austrolebias charrua, a Cyprinodontiforme phylogenetically very distant from the former teleosts. Consistently, here we showed that the ICL and dorsal-medial zone of the OB of G. omarorum contains rostral-caudally oriented cellular processes that are reactive to DCX. This microtubule associated protein is expressed by migrating neuroblasts during development (Francis et al., 1999) up to adulthood in the telencephalon of mammals (Gleeson et al., 1999; Lim et al., 2008; including the rostral migratory stream on humans, Wang et al., 2011), and birds (Boseret et al., 1997). In our knowledge DCX was only demonstrated in the telencephalon and mesencephalon the teleost, Nothobranchius furzeri (Terzibasi et al., 2012).
Nevertheless, other authors demonstrated local proliferation zones at superficial layers of the OB in C. auratus, Barbus meridionalis, Cyprinus carpio, and Salmo gardneri (Alonso et al., 1989), Oreochromis mossambicus (Teles et al., 2012), A. leptorhynchus (Zupanc and Horschke, 1995), and D. rerio (Zupanc et al., 2005) and local migration between layers of the OB.
Our results also support a simultaneous process of radial migration of newborn cells from the proliferation zone nearby rostral subpallium and caudal OB to the surrounding subpallial cell masses, as indicated by the distribution of CldU labeled nuclei (Supplementary Figure 3), similar to the findings of Grandel et al. (2006) in D. rerio.
Other outstanding proliferation and migration processes occurred in the Cb of adult G. omarorum as newborn cells migrated along relatively large distances in all cerebellar divisions (CCb, VCb, and EG) as they relocate from one cerebellar layer to another. There, the migration process involved an almost complete shift of newborn cells between cerebellar layers in a period of 30 days after CldU administration, as previously shown in the Cb of this (Olivera-Pasilio, 2014) and other teleost species (A. leptorhynchus: Zupanc et al., 1996; D rerio: Zupanc et al., 2005; Kaslin et al., 2009; C. auratus: Delgado and Schmachtenberg, 2011; O. mossambicus: Teles et al., 2012; and M. rume: Radmilovich et al., 2016). According to the distribution of DCX cellular process in the CCb of G. omarorum, the migration process of new born cells may involve displacements in the medial-lateral direction along the CCb-mol (as shown by Kaslin et al., 2009), as well as in the rostral-caudal direction in the ganglionic layer, not described previously.
Shorter range or less numerous migration processes were found in other mesencephalic (TeO and OT) and rhombencephalic brain regions (ELL) involved in multimodal and electrosensory information processing. The migration process of newborn cells in the TeO of G. omarorum appeared to occur mainly from the caudal pole of the tectal proliferation zone toward almost all tectal layers as well as from the dorso-medial edge of more rostral zones of the tectal proliferation zone. This involves both the addition of newborn cells to the dorso-medial edge to the tectal proliferation zone, and the displacement of older cells to adjacent caudal parts of the TeO in the ventro-lateral direction as demonstrated in O. latipes (Alunni et al., 2010), C. auratus (Raymond and Easter, 1983) and D. rerio (Ito et al., 2010), and N. furzeri (Terzibasi et al., 2012). Consistently, a net of DCX process lies beneath G. omarorum dorsal-medial tectal proliferation zone.
Neurogenic Potential of Adult G. omarorum Brain Proliferation Zones
After long term chases, the nuclei of most derived cells lost the typical appearance of migrating cells as they reached their target brain regions. Nuclei acquired a rounded shape with heterogeneous distribution of loosely and densely packed chromatin, frequently showing a carriage wheel arrangement of compacted chromatin, as evidenced by thymidine analog labeling. This indicates that these cells are already in the process of cell differentiation that was confirmed by the demonstration of the expression of early or mature neuronal markers, or the retrograde transport of Neurobiotin by long term CldU label retaining cells.
Even though at short chases (1 or 7 days) some derived cells had the aspect of migrating neuroblasts; most of these cells do not express the early neuronal marker DCX, with the exception of few cells nearby the ventral zone of the telencephalic proliferation zone 1b, similar to N. furzeri (Terzibasi et al., 2012). Conversely, 7 days were sufficient for the expression of HuC/HuD by CldU label retaining cells nearby the subpallial proliferation zone, indicating their differentiation into the neuronal phenotype. Some newborn cells nearby the ventricular surface of the subpallial proliferation zone express DCX at a chase duration of 30 days, a slightly longer time interval than observed in mammal hippocampus (Kempermann et al., 2008) and N. furzeri (Terzibasi et al., 2012). This and their morphology indicate that they correspond to migrating neuroblasts. At this chase, other newborn neurons expressing HuC/HuD were located laterally to the subpallial proliferation zone, or rostrally, at the ICL of caudal OB. Longer chases were required for newborn neurons expressing HuC/HuD to reach the ICL of the rostral OB, supporting a long-range migration from the telencephalic ventricle. Strikingly, CldU-HuC/HuD double labeled cells reached more than 50% of newborn migrated cells 90 days after CldU administration. To our knowledge, this has not been reported before, since most of previous studies combining HuC/HuD and thymidine analog retention to demonstrate the differentiation into the neuronal phenotype in the OB failed, either to identify cells expressing HuC/HuD (Zupanc et al., 2005) or the co-localization of HuC/HuD and the thymidine analog (Adolf et al., 2006), or find very few double labeled cells (Grandel et al., 2006). Only the quantitative results of Hinsch and Zupanc (2007) support a 30% fraction of BrdU labeled cells also expressing HuC/HuD after chases between 446 and 656 days.
On the other hand, Alonso et al. (1989) not only found a proliferation zone in the wall of the telencephalic ventricle or ventricular recess but also another at the outer limiting glial membrane and the olfactory nerve fiber layer of C. auratus, B. meridionalis, C. carpio, and Salmo gairdneri. Superficial proliferation zones at the primary olfactory fiber layer and/or the glomerular layer of the OB were also found in other teleost (O. mossambicus: Teles et al., 2012; A. leptorhynchus: Zupanc and Horschke, 1995; D. rerio: Zupanc et al., 2005) that give rise to newborn cells that migrate toward the inner cell layers. Only in O. mossambicus it was shown a high proportion of newborn cells originated from the superficial proliferation zone of the OB expressing HuC/HuD (Teles et al., 2012). All these findings suggest that there are marked interspecific differences in the site of generation, the paths of migration and fate of newborn cells.
A step forward in the process of neuronal differentiation was evidenced by the expression of a more cell specific neuronal marker: TH, the key step-limiting enzyme of the catecholamine synthesis pathway. TH first co-localize with CldU at a chase of 90 days in newborn neurons located within or nearby the subpallial proliferation zone. At 180 chase duration (similar to CldU-HuC/HuD double labeled cells), CldU-TH cells were found further away from the proliferation zones, both in the medial lateral direction (reaching the MOTF and Vc) and in the rostral caudal direction (reaching the ICL of caudal and rostral OB). This is coincident with the results of Grandel et al. (2006) and Adolf et al. (2006) in D. rerio, though in G. omarorum it was not a rare finding. Conversely, according to our quantitative data, newborn catecholaminergic neurons reached 0,5% of migrated newborn neurons of the subpallium 90 days after CldU administration, a figure that was duplicated and triplicated at caudal and intermediate regions of the OB at the longest chase studied (180 days). The population of newborn catecholaminergic neurons was not homogeneous, but showed morphological characteristics corresponding to different steps in the process of cell maturation (from migrating neuroblasts to multipolar granular cells). According to the morphology and location, double labeled CldU-TH newborn cells of the OB of G. omarorum correspond to granule cells of the ICL as shown in other teleosts (Dicentrarchus labrax: Batten et al., 1993; D. rerio: Byrd and Brunjes, 1995; and Solea senegalensis: Rodríguez-Gómez et al., 2000). However, this is not coincident with the distribution of catecholaminergic neurons in the OB of A. leptorhynchus (Sas et al., 1990), D. rerio (Adolf et al., 2006), and D. labrax (Sébert et al., 2008) as in these species TH positive cells are almost absent in the ICL and more abundant in outer layers.
According to our results and, it takes 30 days for newborn cells of the CCb-gra to express the early neuronal marker HuC/HuD, indicating their differentiation into granule cells. This is similar to D. rerio but either much longer (Grandel et al., 2006) or shorter (Kaslin et al., 2009) chase durations were reported, or even absence of double labeling of CCb-gra newborn cells even at very long chase durations (Zupanc et al., 2005). Conversely, in Austrolebias, a 1 day chase is enough for co-localization of BrdU and HuC/HuD (Fernández et al., 2011). These differences may be due to variations in the sensitivity of immunohistochemical procedures, or in the process of cell differentiation because of differences in the durations of life span as argued before.
More than half of newborn CCb-gra cells express HuC/HuD in G. omarorum at 90 day chase duration, a value that amply surpass the fraction of CCb new born cells in D. rerio at 446–656 day chases (2,4%, according to the numbers of BrdU and BrdU-HuC/HuD double labeled cells reported by Hinsch and Zupanc, 2007).
HuC/HuD is also expressed by tectal and toral newborn neurons but requiring longer chases (90–180 days). In D. rerio, double labeled BrdU-HuC/HuD newborn neurons were found nearby the proliferation zone of the TeO (Zupanc et al., 2005; Grandel et al., 2006). The cortical organization of the TeO and the distribution of newborn neurons in almost all its width, suggest the coordinated migration of cohorts of newborn cells of various phenotypes. The fraction of TeO double labeled cells here found in adult G. omarorum also largely exceeds the values in D. rerio according to the quantitative results reported in Hinsch and Zupanc (2007).
We also found newborn double labeled CldU-HuC/HuD neurons in the ELL, though they show weak HuC/HuD immunoreactivity. To our knowledge, the generation of new neurons (by demonstration of HuC/HuD expression in thymidine analog retaining cells) has not been reported neither in the TS nor the ELL of teleosts. It is interesting to note that all these brain regions are involved in sensory information processing, particularly of electrosensory information.
To identify the neuronal phenotype of newborn neurons, we draw upon the combination of repetitive thymidine analog labeling and “in vivo” neuronal tracing to retrogradely label cerebellar and ELL granule cells. This approach rendered a high proportion of granule cells retrogradely labeled, even at distances of more than 200 microns of the site of Neurobiotin application, as well as a high proportion of long term CldU retaining granule cells. These facts probably favored the identification of several double labeled CldU-Neurobiotin granule cells, indicating that these cells already acquired a mature phenotype with axonal projections to the CCb-mol. Similar, though quantitatively much less frequent results were obtained in A. leptorhynchus (Zupanc et al., 1996) and D. rerio (Zupanc et al., 2005) by “ex vivo” retrograde labeling of granule cells with dextran-fluorescein. We did not identify double labeling of any of the other Cb cell types. Finally, unlike the CCb, we did not observe double labeled CldU-Neurobiotin granule cells in the ELL, even though Neurobiotin application to the lateral line nerve rendered abundant trans-synaptic labeled granule cells (data not shown).
In summary, the results of this work confirm the spatial distribution of adult G. omarorum brain proliferation zones, and the migration paths of newborn cells from the proliferation zones to their final locations, particularly at the rostral telencephalon, TeO, TS, and CCb. Our results are compatible with a rostral migratory stream of newborn cells from a proliferation zone at the rostralmost end of the telencephalic ventricle toward the rostral and caudal OB. We also demonstrate widespread and relatively frequent neurogenesis in the telencephalon (subpallium and OB), mesencephalon (TeO and TS), and rhombencephalon (CCb and ELL) of adult G. omarorum. These findings contribute to support the widespread distribution of brain proliferation zones and their neurogenic capacity in G. omarorum, an animal model suitable to assess the functional significance, as well as comparative analysis of adult neurogenesis. Our results also contribute to support the phylogenetically conserved feature of adult neurogenesis. Considering the rough similarity in distribution of brain proliferation zones among teleost species studied up to date, the differences in the neurogenic capacity between the same regions among teleosts suggest differences in the intrinsic/extrinsic factors modulating both cell proliferation and neurogenesis, which is the topic of ongoing research.
MC, ML, and VO made substantial contributions to the conception or design of the work; and/or the acquisition, analysis, and interpretation of data for the work; MC and VO drafted the work. Final approval of the version to be published was done by VO and MC.
This work was partially supported by Agencia Nacional de Investigación e Innovación (Research Grants # FCE_2009_1_2246; FCE_3_2011_1_6168 and ANII fellowship #INI_X_2012_1_4392 to ML), and Programa para el desarrollo de Ciencias Básicas (PEDECIBA).
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.
The authors thank Ranch Los Mojinetes (Laguna del Sauce, Maldonado, Uruguay) for cooperating with this investigation by allowing and assisting with the exploration of the Laguna del Sauce northern coast. The authors also thank to Neurochemistry Department at IIBCE for the generously provide of anti-TH primary AB. We also acknowledge Dr. Milka Radmilovich for helpful reading of the manuscript and fruitful comments and suggestions.
The Supplementary Material for this article can be found online at: https://www.frontiersin.org/article/10.3389/fnins.2017.00437/full#supplementary-material
Supplementary Video 1. Newborn neuron in the olfactory bulb of adult G. omarorum. The video corresponds to an animation obtained with Fluoview from a stack of confocal images obtained from a frontal section of the caudal OB processed for the immunohistochemical detection of tyrosine hydroxilase (green) and CldU (red). The stack consisted in 13 confocal planes, acquired in sequential mode, every 1 μm. Note in the center of the animation a double labeled newborn neuron, corresponding to the cell shown in Figure 10C, as well as other single labeled TH+ or CldU+ cells. Online available at: https://figshare.com/s/0fab179fd0e1e6356371.
Supplementary Video 2. Newborn neuron in the corpus cerebelli of adult G. omarorum. The video corresponds to an animation obtained with Fluoview from a stack of confocal images obtained from a frontal section of the corpus cerebelli (CCb) processed for the immunohistochemical detection CldU (red) and histochemical demonstration of Neurobiotin (green). Note in the right of the animation a double labeled newborn neuron, corresponding to the cell shown in Figure 15B, as well as other single labeled Neurobiotin+ or CldU+ cells. Online available at: https://figshare.com/s/af3f18ae8aea51d80b27.
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Keywords: cerebellum, olfactory bulb, tectum opticum, CldU, doublecortin, HuC/HuD, tyrosine hydroxylase, retrograde tracing
Citation: Olivera-Pasilio V, Lasserre M and Castelló ME (2017) Cell Proliferation, Migration, and Neurogenesis in the Adult Brain of the Pulse Type Weakly Electric Fish, Gymnotus omarorum. Front. Neurosci. 11:437. doi: 10.3389/fnins.2017.00437
Received: 06 April 2017; Accepted: 17 July 2017;
Published: 17 August 2017.
Edited by:Irmgard Amrein, University of Zurich, Switzerland
Reviewed by:Jan Kaslin, Australian Regenerative Medicine Institute (ARMI), Australia
Krishna Vadodaria, Salk Institute for Biological Studies, United States
Satoshi Ogawa, Monash University Malaysia, Malaysia
Copyright © 2017 Olivera-Pasilio, Lasserre and Castelló. 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) or licensor 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: María E. Castelló, firstname.lastname@example.org; email@example.com