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Doublecortin-immunoreactive (DCX+) cells were detected across the allo- and neo-cortical regions in the adult guinea pig cerebrum, localized to layer II specifically at its border with layer I. The density of labeled cells declined with age, whereas no apparent apoptotic activity was detectable over the cortex including layer II. DCX+ cells varied in somal size, labeling intensity, nuclear appearance, and complexity of processes. These cells were often arranged in clusters with cells of similar morphology sometimes packed tightly together. They exhibited complete colocalization with polysialylated neural cell adhesion molecule (PSA-NCAM) and neuron-specific type III β-tubulin (TuJ1). Medium to large-sized DCX+ cells had well-developed neuritic processes, and expressed neuron-specific nuclear protein (NeuN). Large mature-looking cells with weak DCX reactivity invariably displayed heavy NeuN reactivity, implicating a transitional stage of these labeled cells. These “transitional” cells also consistently exhibited weak reactivity for γ-aminobutyric acid (GABA), glutamate decarboxylase (GAD67), β-nicotinamide adenine dinucleotide phosphate diaphorase (NADPH-d) and neuronal nitric oxide synthase (nNOS), suggestive of them being young GABAergic/nitrinergic interneurons. Our data indicate that DCX+ cells exist widely in the adult guinea pig cerebral cortex, with a predominant localization in upper layer II. The morphological variation and differential expression of neuronal markers in these cells implicate that they might be developing neurons, and that they are probably differentiating into GABAergic interneurons. This population of cells might be involved in interneuron plasticity in the adult mammalian cerebral cortex.
In the developing brain, doublecortin (DCX) appears to play a crucial role in neuronal migration (Francis et al., 1999), including tangential migration of interneuron precursors into the cortex (Friocourt et al., 2007). A DCX gene mutation is related to X-linked subcortical laminar heterotopia (“double cortex” syndrome), a subclass of lissencephaly characterized by mental retardation and epilepsy ([des Portes et al., 1988] and [Gleeson et al., 1988]). In the adult brain, newly generated neurons in the hippocampal formation and the subventricular zone express DCX ([Magavi et al., 2000] and [Nacher et al., 2001]). Thus, DCX is transiently present in immature neurons that eventually develop into mature granule cells and integrate into functional hippocampal circuitry (Brown et al., 2003). Similarly, DCX immunoreactive (DCX+) neuroblasts in the subventricular zone migrate via the rostral migratory stream and differentiate into mature GABAergic interneurons in the olfactory bulb ([Magavi et al., 2000], [Nacher et al., 2001] and [Gritti et al., 2002]).
A novel population of DCX+ cells has been reported in the temporal and prefrontal cortices of mice, rats and primates. These cells reside primarily in layer II, and invariably express several other molecules enriched in immature neurons, including polysialylated neural cell adhesion molecule (PSA-NCAM) and neuron-specific tubulin-III (TuJ1)([Seki and Arai, 1991], [Bonfanti et al., 1992], [O'Connell et al., 1997], [Fox et al., 2000], [Nacher et al., 2001] and [Varea et al., 2007a]). The true identity and origin of these cortical DCX+ cells remains elusive, and little is known regarding their existence in other mammalian species apart from those mentioned above (Bonfanti, 2006). Also, unlike adult-born subgranular and subventricular cells that express the very same set of immature neuronal markers, considerable controversy remains as to whether these DCX+ cortical cells are newly generated. For example, findings of 5-bromo-2′-deoxyuridine (BrdU) incorporation in these cells have been mixed ([O'Connell et al., 1997], [Fox et al., 2000], [Nacher et al., 2001], [Nacher et al., 2004], [Bernier et al., 2002], [Varea et al., 2005], [Bonfanti, 2006], [Pekcec et al., 2006], [Shapiro et al., 2007a] and [Shapiro et al., 2007b]).
In the present study, we have identified DCX+ cells in layer II throughout the allo- and neo-cortical areas in the adult guinea pig. Based on their morphology and differential expression of immature and mature neuronal markers, these DCX+ cells appear to be immature neurons undergoing differentiation. Moreover, some mature-looking DCX+ cells co-express γ-aminobutyric acid (GABA), glutamate decarboxylase (GAD67), β-nicotinamide adenine dinucleotide phosphate diaphorase (NADPH-d) and neuronal nitric oxide synthase (nNOS). The existence of this population of neurons in the adult cerebral cortex might have important functional implications, potentially regarding interneuron plasticity under physiological conditions as well as interneuron alterations under certain pathophysiological circumstances.
Male Hartley guinea pigs weighing 560–1250 g were purchased from Charles River Laboratories (Wilmington, MA). Animals at 3, 6, 12, 24 and 36 months-old (n = 4 per age) were used to quantify the densities of DCX+ cells. Colocalization studies were carried out in brain sections from 6 and 12 months-old animals. Additional 3 (n = 3) and 12 (n = 3) months-old animals were used for western analyses and in situ detection of DNA cleavage, together with frozen adult (2 months-old) rat brains (n = 3) and olfactory bulb sections (n = 3) available from a recent study serving as materials for positive controls (Yan et al., 2007).
For immunohistological studies, guinea pigs were perfused via the ascending aorta with 4% paraformaldehyde with (for GABA immunolabeling) or without 0.5% glutaraldehyde in 0.01 M phosphate-buffered saline (pH 7.4, PBS) under overdose anesthesia (sodium pentobarbital, 100 mg/kg, i.p.). Brains were removed, postfixed overnight, and soaked in 30% sucrose in PBS at 4 °C until they sunk. One cerebral hemisphere from each brain was sectioned coronally using a cryostat. Twenty consecutive sections at 30 μm thickness in every 1 mm of brain were serially collected into culture plates. From the septal to mid-hippocampal levels, approximately 20 sets of 8 μm sections were also collected, and thaw-mounted on positively charged microslides (VWR International, West Chester, PA). Tangential cortical sections were prepared from some brains using the other hemisphere. The cortex was separated from the striatum and hippocampal formation, and flat-embedded between Parafilm pieces lining inside two microslides. The flattened cortex was cut at 8 or 30 μm from the pial surface down. All 30 μm sections were used for immunolabeling using the peroxidase method, while double immunofluorescence was carried out on 8 μm sections. One set of the 30 μm sections was processed with Nissl stain for histological orientation. For western analyses and in situ detection of DNA cleavage, brains were rinsed briefly by perfusion with cold PBS. Semi-brains (forebrain hemispheres) from each animal were then snap-frozen for protein extraction and slide-mounted cryostat sections at 20 μm (coronal), respectively.
Animal use was in accordance with the National Institute of Health Guide for the Care and Use of Laboratory Animals. All experimental procedures in the present study were approved by the Institutional Animal Care and Use Committee of Southern Illinois University Carbondale.
To visualize immunoreactivity with the peroxidase method, sections were treated initially with 1% H2O2 in PBS for 30 min, and then in 10% normal rabbit serum in PBS with 0.3% Triton X-100 for 1 h at room temperature. Subsequently, sections were incubated in PBS containing goat anti-DCX (1:2000) (see Table 1), 5% normal rabbit serum and 0.1% Triton X-100 overnight at 4 °C. Sections were further reacted with biotinylated rabbit anti-goat IgG at 1:400 for 2 h, and subsequently with ABC reagents (1:400) (Vector Laboratories, Burlingame, CA) for 1 h. Immunoreaction products were visualized using 0.003% hydrogen peroxide and 0.05% diaminobenzidine. Three 10-minute washes with PBS were used between incubations. Sections were mounted on slides, allowed to air-dry, and then were dehydrated, cleared and coverslipped.
For immunofluorescence, slide-mounted sections (8 μm thick) were incubated in PBS containing 5% donkey serum, 0.3% Triton X-100 and a pair of primary antibodies raised in different species overnight at 4 °C (see Table 1). Sections were further incubated for 2 h at room temperature in PBS containing Alexa-Fluor® 488 and Alexa-Fluor® 568 conjugated donkey antibodies against mouse, rabbit or goat IgGs (1:200, Invitrogen, Carlsbad, CA). Sections were finally counter-stained with bisbenzimide (Hoechst 33342, 1:50,000), washed and coverslipped with anti-fading medium (Vector Laboratories).
The primary antibodies applied in this study have been used in multiple previous reports (See Results). In the present study, omission of the antibody in the assay buffer or substitution with a corresponding normal serum yielded no specific labeling.
β-Nicotinamide adenine dinucleotide phosphate diaphorase (NADPH-d) histochemistry was carried out as described previously (e.g., Yan et al., 1994). In brief, sections were incubated in a solution containing 0.3% Triton X-100, 1 mM β-NADPH-d (N7505, Sigma-Aldrich, St. Louis, MO), 0.8 mM nitroblue tetrazolium (N6639, Sigma-Aldrich) and 5% dimethyl sulfoxide in 0.05 M Tris–HCl buffered saline (pH 8.0, TBS) for 15 or 45 min at 37 °C. The reaction was stopped by rinsing sections in PBS. Some sections were further processed for DCX or NOS immunolabelings using the peroxidase method as described above.
A modified terminal deoxynucleotidyl transferase-mediated nick end labeling (TUNEL) assay was performed as described (Yan et al., 2001). Fresh-frozen guinea pig cortical and rat olfactory bulb sections (20 μm) were fixed with 4% paraformaldehyde at room temperature in PBS for 20 min. The olfactory bulb sections were from rats surviving 1 month post unilateral naris-occlusion (Yan et al., 2007), serving as ideal positive control for TUNEL since apoptosis exists in normal rodent bulbs but increases significantly following functional deprivation (Najbauer and Leon, 1995). Slide-mounted sections were treated with 0.3% Triton X-100 in PBS for 30 min, rinsed in distilled water for several minutes, and incubated with 0.06 U/ml terminal deoxynucleotidyl transferase (TDT, Amersham Biosciences, Piscataway, NJ, E2230Z), and 4 mM biotin-16-dUTP (Roche Diagnostics, Indianapolis, IN, 11-093-070-910) in TDT buffer (pH 7.4, containing 140 mM sodium cacodylate, 1 mM cobalt chloride in PBS) at 37 °C for 3 h. The DNA terminal labeling was visualized with Alexa-Fluor 568-conjugated streptavidin (Invitrogen, 1:500), followed by bisbenzimide counterstain for laminar orientation.
The piriform and entorhinal cortices of the guinea pigs and rats were dissected out and homogenized with a sonication device in T-PER buffer (10× w/v) (Pierce, Rockford, IL) containing a cocktail of protease inhibitors (Roche). Tissue lysates were centrifuged at 8000 ×g at 4 °C for 10 min. Supernatants were collected and protein concentrations determined by DC protein assay (Bio-Rad Laboratories, Hercules, CA). Equal quantities of protein (30 μg) were run on 10% SDS-PAGE gels (Hoefer Scientific Instruments, San Francisco, CA). The polypeptides were electrotransferred to Trans-Blot® pure nitrocellulose membrane (Bio-Rad Laboratories). Non-specific binding was blocked with PBS containing 5% nonfat milk and 3% bovine serum albumin. Nitrocellulose membranes were blotted overnight with goat anti-DCX (1:2000) and rabbit anti-doublecortin-like kinase 1 (1:500) antibodies, respectively (see Table 1), followed by incubations in HRP-conjugated secondary antibodies (1:5000, Bio-Rad Laboratories) for 1 h. Protein bands were visualized with an ECL Plus™ Western Blotting Detection kit according to manufacturer's instruction (GE Healthcare Life Sci., Piscataway, NJ), and images captured immediately in a UVP Biodoc-it™ system (UVP, Inc, Upland, CA). Equal protein loading was evaluated by re-blotting β-tubulin-III signal (1:20,000) on the same membranes.
Sections were examined and imaged on an Olympus fluorescent BX60 microscope equipped with a digital imaging system (MicroFire® CCD Camera and software, Optronics, Goleta, CA). For cell counts, three coronal sections at comparable rostrocaudal levels were selected. Camera lucida drawings of labeled cells were made along the pial surface. Using the rhinal fissure (RS) and lateral sulcus (LS) as landmarks, the cortex was divided into parietal, temporal, entorhinal and piriform areas. Dots representing labeled cells were counted in each cortical segment, with the lengths of the pial surface measured for corresponding cortical segments. Cell density was calculated and expressed as the number of cells per millimeter length of pial surface. Images of representative sections were captured using a 10× objective, and subsequently montaged with Photoshop 7.0.
Immunofluorescent labelings in coronal or tangential sections were examined with 20× and 40× objectives. Images of the same cellular profiles were taken using green (DCX labeling), red (other immunolabelings) and blue (bisbenzimide stain) fluorescent filters. Some sections were also examined with a confocal microscope (Olympus Fluoview, Japan), and overlapping of labeled cells was rarely encountered in the 8 μm sections.
Means of cell densities were calculated for individual and groups of animals. Statistical comparisons were conducted using one-way ANOVA followed by Bonferroni's pair-wise comparisons, yielding p values between individual groups (Prism GraphPad 4.1, San Diego, CA). The minimal significance level was set at p < 0.05. All illustrations were prepared with Corel Draw 10 (Corel Corp., Ontario, Canada). Whole panel images were converted into a TIFF format, with contrast/brightness adjusted as needed.
To confirm the specificity of the goat anti-DCX antibody used in the preset study, western analyses were carried out using both guinea pig and rat cerebral extracts (piriform/entorhinal cortex). As with previous reports ([Brown et al., 2003] and [Capes-Davis et al., 2005]), this antibody recognized a single band migrated at ~ 40 kd in cortical lysates from both species (Fig. 1). In the same cortical samples, a putative doublecortin-like kinase-1 protein visualized with an antibody from Chemicon (Table 1) migrated at ~ 85 kd, consistent with the predicted molecular size of this latter protein (Capes-Davis et al., 2005). Thus, the expression of DCX in the brain appeared similar for rat and guinea pig, and the goat antibody appeared to be highly specific to DCX in these two species.
DCX+ cells were found in multiple forebrain areas of all adult guinea pigs examined in the present study (Fig. 2). Consistent with previous findings in other species, DCX+ cells occurred in the rostral migratory stream (Fig. 2A, C), the subventricular zone as well as the nearby white matter (Fig. 2D, F, H), and the subgranular zone of the hippocampal dentate gyrus (Fig. 2H, J).
Distinct DCX+ cells were also seen in the cerebral cortex in the superficial region of the cortical mantle, forming a cellular band deep to layer I throughout the allo- and neo-cortical areas (Fig. 2A, D, H). Radially this band included a few cells in layer II, primarily at the border with layer I. Individual DCX+ cells were also noted in the upper part of layer III (especially in the piriform and entorhinal cortices) (Fig. 2B, E, I, K). For descriptive simplicity and consistency with literature, we refer to these cells collectively as layer II DCX+ cells in this current study. Tangentially this cellular band continued beneath the pial surface over the medial, dorsal and lateral cerebral aspects (Fig. 2 and Fig. 3). Within a given brain, the abundance of DCX+ cells in various cortical regions varied, with an approximate order of labeling being from high to low: piriform, entorhinal, temporal/frontal, and parietal/occipital areas (Fig. 2 and Fig. 3).
To determine whether there was an age-dependent change in DCX+ cell population, the density of immunoreactive cells was quantified in the parietal, temporal, entorhinal and piriform areas using 3 sections (~ 2 mm apart) at the rostral to middle hippocampal levels from each animal (Fig. 3). To accomplish this, sections from individual animals were processed in parallel using multiple-chambered incubators. An overall decline of DCX+ cells was found with age in all neo-and allo-cortical areas analyzed (F = 19.29 for piriform, 32.80 for entorhinal, 51.37 for temporal and 39.32 for parietal cortices, respectively, with p < 0.0001 and df = 4, 10 in all cases, one-way ANOVA) (Fig. 3B). In all areas except the parietal cortex (p < 0.01), the mean densities of DCX+ cells in 3 months-old animals were not statistical different than that seen at 6 months, although differences were noted relative to older animals (p < 0.001 to p < 0.0001). Similarly, the mean densities at 6 months were not significantly different from that at 12 months, but again, were significantly different relative to those at 24 and 36 months. Further, the densities at 12 months did not reach statistical significance as compared to those of 24 (p = 0.067) and 36 months (p = 0.052).
To explore whether the age-related decline in layer II DCX+ cells might involve obvious cell death or apoptosis, we carried out TUNEL assay in cortical sections from 3 (Fig. 4A, B) and 12 (not shown) months-old guinea pigs. At both ages, TUNEL profiles were occasionally encountered over the cortex and white matter, without noticeable laminar preference (Fig. 4A, B). In particular, there was no apparent indication of elevated TUNEL activity in layer II and its vicinity relative to the rest laminae of cortex. In contrast, in the rat olfactory bulb sections processed under identical conditions, TUNEL activity was evident across the sections especially the granule cell layer. Further, labeled profiles were apparently denser in the deprived side relative to the non-deprived side (Fig. 3C), as demonstrated previously (Najbauer and Leon, 1995). Because of the rare occurrence of TUNEL profiles across the normal guinea pig cortex (especially in layer II), a comprehensive search and analysis for double labeling of TUNEL and DCX was not performed in this study.
Overall, layer II DCX+ exhibited a heterogeneous morphology (Fig. 5). Cell bodies exhibited various shapes, including round, oval, bipolar, multipolar, pyramidal-like and irregular (Fig. 5A–E). The smallest cells were approximately 5 μm in somal diameter, weakly stained, and had no, one/two processes that extended from one or opposite poles of the somata. Other small cells were often bipolar with stronger labeling and longer processes (Fig. 5 and Fig. 6). Medium-sized (5–10 μm) cells displayed moderate to heavy DCX reactivity, with 2–4 processes radiating from the somata and extending for up to 100 μm into layer II and the lower part of layer I. Large-sized DCX+ cells ranged from approximately 10–20 μm in somal diameter and had branched dendrite-like processes that extended tangentially, obliquely or radially for several hundred micrometers (Fig. 5A–E). These branches could often be traced to the pial surface (Fig. 2 and Fig. 5). Thin, axon-like processes were identifiable on many medium and large-sized DCX+ cells. These axons extended into the deeper cortical layers frequently reaching as far as layer IV (Fig. 5B, C). Most of the large DCX+ cells showed moderate staining intensity, whereas a subpopulation of these cells displayed apparently reduced immunoreactivity in both the somata and processes (Fig. 5 and Fig. 6). Overall, small DCX+ cells appeared to outnumber medium and large-sized cells in any given region, which was most noticeable at the interface between layers I and II in tangential sections (Fig. 5D).
DCX+ cells appeared to occur in clusters, which was apparent in tangential sections. No obvious regularity or consistency was recognizable with regards to cell number, size, shape, or the border and distance between individual clusters (Fig. 2 and Fig. 5). However, within a given cluster cells of different sizes and shapes often co-existed (Fig. 5D, E). In many cases, a pair or several labeled somata were tightly packed together or appeared to be physically attached. These closely apposed cells often displayed comparable morphological features (i.e., similar somal diameter, staining intensity, dendritic arbor size and nuclear appearance) (Fig. 2, Fig. 5 and Fig. 6).
In bisbenzimide stained sections, small DCX+ cells had small but brightly stained nuclei that were almost as big as their somata (Fig. 6A–D, H). Medium to large-sized DCX+ cells had larger but less intensely stained nuclei that were surrounded by a greater amount of cytoplasm (Fig. 6 and Fig. 7). The nuclei of large cells with reduced or faint DCX labeling had a similar appearance to neighboring mature neurons as assessed by other markers (see below) (Fig. 6 and Fig. 7).
Eight micrometer slide-mounted sections that exhibited minimal cellular overlapping were used to determine colocalizations of DCX and other molecules. In general, all layer II DCX+ cells were immunoreactive for PSA-NCAM ([Seki and Arai, 1991] and [Nacher et al., 2002]). PSA-NCAM immunoreactivity tended to outline the somata and dendrites of DCX+ cells. Thus, colocalization of these two markers was most obvious near the plasmalemma (Fig. 6A–D). Complete DCX colocalization with neuron-specific type III β-tubulin (TuJ1 or Tu-20) was also noted in this population of cells (Fig. 6E) (Yan et al., 2001).
To determine whether Cajal–Retzius cells or astrocytes could contribute to the layer II DCX+ cells, double labeling for DCX and reelin or GFAP was performed (Gong et al., 2007). As illustrated in Fig. 6F, reelin and DCX did not colocalize in layers I and II. Also, no colocalization of DCX with GFAP was noted in any cell (Fig. 6G).
DCX+ cells showed variable immunoreactivity for NeuN (Fig. 6H–K) (Yan et al., 2001). Specifically, small DCX+ cells, whether individually distributed or tightly packed, did not express NeuN (Fig. 6H–K). In contrast, larger DCX+ cells consistently expressed NeuN (Fig. 6I–K). Among the medium-sized DCX+ cells, weak NeuN labeling was seen in the nuclei of some cells but not others (Fig. 6I–K). Thus, it appears that elevated NeuN levels are concordant with a decrease in DCX staining in medium to large somal sized cells.
Many DCX+ cells exhibited a mature-looking neuronal morphology and expressed high levels of NeuN. Thus, we examined whether specific markers of principal or local circuit neurons were present in these cells. Neurogranin, a neuron-specific protein that is heavily and exclusively expressed in cerebral principal neurons (Singec et al., 2004), was not colocalized with DCX+ cells, including those with weak or faint DCX reactivity (Fig. 7A–D).
A subpopulation of DCX+ cells however displayed weak to moderate GABA labeling (Yan et al., 1996b). In general, GABA immunoreactivity was not observed in small DCX+ cells, but became consistently detectable in most medium and large-sized cells (Fig. 7E–G). In fact, strong and distinct GABA reactivity occurred in virtually all large cells with weak DCX reactivity. Similarly, large-sized mature-looking cells with reduced DCX levels co-expressed GAD67 (Fig. 7H–N) or GAD65/67 (not shown but with similar patterns as GAD67) (Yan et al., 1998). Of note, GAD reactivity in DCX+ cells was weak relative to nearby, presumably mature, interneurons that displayed only GAD but no DCX labeling. Also, colocalization of DCX and GAD was better viewed in tangential sections (at the immediate interface of layer I and II) over areas with less crowded neurons and less dense GAD labeling in the neuropil (Fig. 7K–N). No clear colocalization of DCX and calcium-binding proteins (parvalbumin, calbindin and calretinin), markers of mature GABAergic subpopulations, was however noted (not shown).
Nitric oxide synthase (NOS) is expressed in subpopulations of cortical interneurons, and can be detected by NADPH-d histochemistry or NOS immunolabeling (Dawson et al., 1991). Type I nitrinergic neurons have a large somal size and exhibit heavy NADPH-d staining (thus giving the cells a Golgi-like appearance). These cells are few in number and are localized overwhelmingly to the subcortical white matter. Type II neurons have small somal size, light to moderate NADPH-d reactivity, and are numerous in the supragranular cortical layers ([Yan et al., 1996b] and [Smiley et al., 2000]; review by Judas et al., 1999).
Some layer II DCX+ cells displayed weak yet consistent NADPH-d or neuronal NOS (nNOS) reactivity (Fig. 8). As with GAD67, NADPH-d or nNOS labeling was observed in large-sized mature-looking neurons that exhibited weak DCX reactivity (Fig. 8A–I). Double-labeled neurons were sometimes close to or apparently attached to each other, or to cells displaying strong and distinct reactivity for either NADPH-d/nNOS or DCX (Fig. 8C–F, I). Of note, all of these NADPH-d/nNOS reactive cells, whether or not expressing DCX, fell into the category of type II nitrinergic neurons. Colocalization of NADPH-d and nNOS in type I and type II nitrinergic neurons was verified in the present study using double labeling (Fig. 8J, K). Type I cells were visualized following a short (15 min) NADPH-d incubation (longer reaction results in heavy nitroblue tetrazolium deposits that mask immunoreaction products).
Most type II NADPH-d neurons also express calbindin ([Yan et al., 1996b], [Yan and Garey, 1997] and [Smiley et al., 2000]). To investigate why there can be a partial colocalization of DCX with NADPH-d but no colocalization with calbindin, the cellular pattern of calbindin/NADPH-d colocalization was examined. Calbindin was found to occasionally colocalize in weak NADPH-d reactive neurons cells, especially those in layers II and III (Fig. 8L). For quantitative analysis, cell counting was conducted in 3 coronal sections from the septal to mid-hippocampal levels in each brain over the parietotemporal areas by scanning along the border of layers I and II at 40× (covering ~ 200 μm cortical depth, roughly corresponding to layer II). These analyses yielded a small degree of calbindin colocalization in NADPH-d neurons (mostly weak reactive) in this lamina, about 9.3% (57/612) and 8.3% (43/516) at 6 (n = 4) and 12 (n = 4) months of age, respectively. In contrast, calbindin reactivity was present in virtually all NADPH-d (mostly moderate reactive) type II neurons in deeper cortical layers (Fig. 8 L, M), as characterized previously ([Yan and Garey, 1997] and [Smiley et al., 2000]).
In the present study a population of DCX+ cells has been characterized in the cerebral cortex of adult guinea pigs. These DCX+ cells are predominately localized to upper layer II (occur from deep layer I to upper layer III). The number of these cells declines from juvenile to older adult stages. These cells co-express PSA-NCAM and TuJ1, two additional molecules that are typically associated with immature neurons. They also differentially express selective mature neuronal markers, but do not express glial marker proteins. These data support the general notion that these DCX+ cells have a neuronal identity ([Seki and Arai, 1991], [Bonfanti et al., 1992], [O'Connell et al., 1997], [Fox et al., 2000], [Nacher et al., 2001] and [Bonfanti, 2006]).
Layer II DCX+ cells exhibited remarkably heterogeneous yet apparently correlated morphological characteristics. From small to larger cells, somal shape ranges from round/oval to bipolar, multipolar or irregular; nuclei evolve from small to large and from bright to pale in bisbenzimide stain; dendrite-like processes increase in number, length and branching complexity; and axon-like processes elongate and extend to deeper cortical layers. These morphological variables observed across DCX+ cells are largely comparable to those characterized in developing cortical neurons in vivo and in vitro ([del Rio et al., 1992], [de Lima and Voigt, 1997] and [Ang et al., 2003]). Thus, it is plausible that layer II DCX+ cells may be immature and developing.
Consistent with this hypothesis, the relative levels of DCX and NeuN in individual cells correlate with somal size and the complexity of neuritic processes. Thus, DCX expression appears to increase as the cells become larger and more mature-looking, until some peak point which is followed by downregulation. On the other hand, NeuN expression emerges in the cells approximately around the stage of peak DCX expression, and increases as DCX levels subsequently decline. DCX and NeuN expression patterns among the labeled cells are consistent with a transient expression of immature and increase of mature neuronal markers in developing neurons ([Brown et al., 2003] and [von Bohlen Und Halbach, 2007]). Taken together, these data suggest that layer II DCX+ cells are undergoing differentiation and maturation.
Also in supportive of a developmental nature of these cells is the lack of apparent indication of elevated apoptosis in layer II in TUNEL assay. Thus, it appears that layer II DCX+ cells might not be inevitably vulnerable to cell death under normal physiological conditions. As positive TUNEL activity is probably only detectable during a short period of time in the course of cell death, one cannot exclude the possibility that a few or some of layer II DCX+ cells may die. Regardless, apoptosis does not appear to be the major or immediate fate of these cortical DCX+ cells.
Layer II DCX+ cells in rodent and primate cortex have been designated as neurogliaform, fusiform, semilunar, semilunar–pyramidal transitional and multipolar neurons, common morphological terms of major cortical interneuron subtypes ([Seki and Arai, 1991], [Nacher et al., 2001], [Bernier et al., 2002] and [Bonfanti, 2006]). We show here that a subpopulation of these DCX+ cells in the adult guinea pig cortex display neurochemical properties of mature cortical interneurons. Specifically, GABA, GAD67, NADPH-d and nNOS reactivities occur in large-sized and morphologically mature-looking cells that exhibited attenuated levels of DCX. In contrast, these interneuron markers are not detectable in small and morphologically primitive cells. In fact, when somal size and the complexity of neuritic branches are taken into account, the differential colocalization pattern of GABA and DCX is largely comparable with that of NeuN and DCX across individual cells. These data implicate that these DCX+ cells are undergoing differentiation into GABAergic/nitrinergic during morphogenesis. The intensity of GABA, GAD67, NADPH-d or nNOS labeling is apparently weaker in DCX double-labeled cells relative to neighboring mature interneurons lacking DCX. Also, calcium-binding proteins (parvalbumin, calbindin and calretinin) are not colocalized with DCX in layer II. Taken together, DCX+ cells co-expressing selective interneuron markers are probably at a transitional stage of development, evolving from immature neurons to young GABAergic interneurons.
In general, more than 90% of type II NADPH-d neurons in mammalian neocortex contain calbindin ([Yan et al., 1996b], [Yan and Garey, 1997] and [Smiley et al., 2000]). As calbindin is not detected in DCX+ cells, we speculate an infrequent colocalization of calbindin in NADPH-d reactive neurons in layer II relative to the overall population of these nitrinergic neurons in the cortex, which is confirmed by quantitative analysis in the present study. One may hypothesize that DCX+/NADPH-d+ cells may further develop into NADPH-d+/calbindin+ neurons in the guinea pig cortex.
BrdU incorporation in layer II DCX+ cells or alike (i.e., PSA-NCAM+ cells) has been described in rodent piriform cortex and monkey temporal lobe cortex ([Bernier et al., 2002], [Pekcec et al., 2006], [Shapiro et al., 2007a] and [Shapiro et al., 2007b]). However, others report little BrdU incorporation in this population of cells ([O'Connell et al., 1997], [Fox et al., 2000], [Nacher et al., 2001], [Nacher et al., 2002], [Nacher et al., 2004], [Varea et al., 2005] and [Bonfanti, 2006]). Of interest, significant changes in the number or density of this group of cells are reported in the piriform, temporal and prefrontal cortex under various experimental conditions, implicating a likelihood of alteration in cell population ([O'Connell et al., 1997], [Fox et al., 2000], [Tonchev et al., 2003], [Nacher et al., 2002], [Nacher et al., 2004], [Sairanen et al., 2007], [Shapiro et al., 2007a], [Varea et al., 2007b] and [van der Borght and Brundin, 2007]). Future studies with improved birth-dating methodology might potentially clarify whether these DCX+ cells are newly-formed in the adult mammalian cortex. Alternatively, they may represent a reservoir of early-formed cells somehow maintaining at relatively immature status over time but capable for structural plasticity under various physiological and perhaps pathophysiological conditions ([Nacher et al., 2001] and [Bonfanti, 2006]).
In the present study, DCX+ cells are found broadly across the guinea pig cerebral cortex including all neo-cortical areas. Morphologically primitive to fairly mature-looking DCX+ cells are essentially restricted to layer II, with virtually no similar cells detectable in deep cortical layers. Therefore, there exists little indication for a direct radial migration of these DCX+ cells from the subventricular zone before they reside in layer II.
During the past decade, it has become clear that cortical interneurons originate mostly from subcortical structures (medial, caudal and lateral ganglionic eminences, and olfactory primordium), with their precursors invading the cortex by tangential migration, including via layer I ([Lavdas et al., 1999], [Wichterle et al., 1999], [Anderson et al., 2001], [Zecevic and Rakic, 2001] and [Ang et al., 2003]). Several studies also show that some interneuron subgroups (including type II nitrinergic neurons) may populate over the cortical plate outside-in ([Soriano et al., 1992], [Yan et al., 1996a], [Wichterle et al., 1999], [Hevner et al., 2004] and [Rymar and Sadikot, 2007]). Importantly, the marginal zone/layer I may play a role in neurogenesis in the cortex during development, potentially contributing GABAergic interneurons to the cortical plate ([Zecevic and Rakic, 2001] and [Costa et al., 2007]). It is interesting to speculate that layer II DCX+ cells may have a local origin, being related to intrinsic layer I neuronal progenitors or interneuron precursors arrived by tangential migration via layer I. This hypothesis appears in harmony with their novel laminar location (at the border of layers I and II) and their potential to differentiate into type II NADPH-d neurons, possibly a phylogenetically and ontogenetically late-appearing GABAergic subpopulation ([Yan et al., 1996a], [Yan et al., 1996b] and [Yan et al., 1996b]).
In summary, this study describes an intriguing group of layer II cells over the adult guinea pig cerebral cortex that expresses DCX and other markers characteristic of immature neurons. There is a trend for morphological maturation of these DCX+ cells that is correlated with neurochemical differentiation into presumptive GABAergic interneurons. The precise origin and destiny of these cells, and their significance in cortical development, maintenance and function, remain a compelling question in neurobiology.
This study was supported by Southern Illinois University (X.X.Y.), Illinois Department of Public Health (X.X.Y., R.W.C., R.G.S.) and Epilepsy Foundation (P.R.P). We thank Dr. Charles E. Ribak at University of California Irvine for his constructive comments on the manuscript.