Skip to main content

Spatiotemporal development of spinal neuronal and glial populations in the Ts65Dn mouse model of Down syndrome



Down syndrome (DS), caused by the triplication of chromosome 21, results in a constellation of clinical features including changes in intellectual and motor function. Although altered neural development and function have been well described in people with DS, few studies have investigated the etiology underlying the observed motor phenotypes. Here, we examine the development, patterning, and organization of the spinal cord throughout life in the Ts65Dn mouse, a model that recapitulates many of the motor changes observed in people with DS.


Spinal cords from embryonic to adult animals were processed for gene and protein expression (immunofluorescence) to track the spatiotemporal development of excitatory and inhibitory neurons and oligodendroglia. Postnatal analyses were focused on the lumbar region due to the reflex and gait abnormalities found in Ts65Dn mice and locomotive alterations seen in people with DS.


Between embryonic days E10.5 and E14.5, we found a larger motor neuron progenitor domain in Ts65Dn animals containing more OLIG2-expressing progenitor cells. These disturbed progenitors are delayed in motor neuron production but eventually generate a large number of ISL1+ migrating motor neurons. We found that higher numbers of PAX6+ and NKX2.2+ interneurons (INs) are also produced during this time frame. In the adult lumbar spinal cord, we found an increased level of Hb9 and a decreased level of Irx3 gene expression in trisomic animals. This was accompanied by an increase in Calretinin+ INs, but no changes in other neuronal populations. In aged Ts65Dn animals, both Calbindin+ and ChAT+ neurons were decreased compared to euploid controls. Additionally, in the dorsal corticospinal white matter tract, there were significantly fewer CC1+ mature OLs in 30- and 60-day old trisomic animals and this normalized to euploid levels at 10–11 months. In contrast, the mature OL population was increased in the lateral funiculus, an ascending white matter tract carrying sensory information. In 30-day old animals, we also found a decrease in the number of nodes of Ranvier in both tracts. This decrease normalized both in 60-day old and aged animals.


We show marked changes in both spinal white matter and neuronal composition that change regionally over the life span. In the embryonic Ts65Dn spinal cord, we observe alterations in motor neuron production and migration. In the adult spinal cord, we observe changes in oligodendrocyte maturation and motor neuron loss, the latter of which has also been observed in human spinal cord tissue samples. This work uncovers multiple cellular perturbations during Ts65Dn development and aging, many of which may underlie the motor deficits found in DS.


Down syndrome (DS) is one of the most prevalent developmental disorders world-wide and is caused by trisomy of human chromosome 21 (Hsa21). In the USA, DS occurs with an incidence of approximately 1 in 792 live births [17, 38], making it the most common genetic cause of intellectual disability and developmental delay [42, 47, 74]. Motor deficits are a common feature of DS and are often apparent at birth. Infants with DS show delays in acquiring both fine and gross motor skills [15] and in many cases these deficits persist throughout life. In particular, infants and toddlers with DS are delayed in achievement of motor milestones including grasping, rolling, sitting, standing, walking, and speaking [44, 49, 57]. While these milestones are achieved in the same order as in typically developing individuals [49, 70], the delays in their acquisition lengthen with age and in accordance with task complexity [44, 51]. Longer reaction and movement times [29, 31] and co-contraction of agonist and antagonist muscle pairs [29] are all characteristic of DS and lead to imprecise and poorly coordinated movements [31]. In addition, individuals with DS have decreased control of grip strength and an inability to adapt grip to environmental changes [13]. Gait and other forms of stereotyped motion are affected as well; infants with DS start walking later than their typically developing peers and can exhibit altered gait throughout life [57]. In general, all central nervous system and behavioral changes in DS, including those impacting the motor system, are ultimately due to the triplication of Hsa21 and the dosage imbalance of Hsa21 genes; however, how these genome changes affect motor function is unknown. Understanding the underlying cause(s) of the motor deficits in DS could identify targets and possible corrective therapies for a more favorable motor outcome.

Several regions of the CNS may play a role in these motor deficits, and multiple anatomical pathways and genes have been implicated. The spinal cord (SC) is an attractive anatomical candidate for the observed motor deficits in DS because both locomotion and tonic control rely on neural circuits that lie within the spinal cord and are, therefore, relatively independent from higher cortical areas [13]. Although the SC is likely affected in people with DS, only one study has investigated SC degeneration in individuals with DS and in mouse models, reporting a decrease in the motor neuron population with age [72]. This finding highlights the need for a more in-depth longitudinal characterization of SC development, cytoarchitecture, and function in DS.

Thus far, trisomy has been shown to impact proliferation, leading to cell allocation defects throughout the developing cerebral cortex, hippocampus, ganglionic eminence, and cerebellum [5, 10, 14, 25, 59]. Furthermore, a strong link between gene dosage and altered brain development in DS has been found with the Oligodendrocyte transcription factor 2 (Olig2) gene, which is triplicated in DS. In addition to a newly discovered role of OLIG2 in a subset of astrocytes [66], OLIG2-expressing precursors in the forebrain generate both inhibitory interneurons (INs) and oligodendrocytes (OLs). Changes in the number and maturation status of both these cell types have been found in trisomic mouse and human forebrain samples [5, 6, 10, 32, 47, 62]. Regarding the affected anatomical pathways, pre- and postnatal post-mortem studies show that people with DS have disproportionately smaller cerebellum compared to typically developing individuals [4, 27, 52], indicating that volumetric changes in this region may be partially responsible for both deficits in motor function and motor learning in people with DS [1, 18, 21, 67]. Seminal work in the Ts65Dn mouse model implicates reduced responsiveness to Sonic Hedgehog (SHH) as a potential cause for this cerebellar hypoplasia [16]. However, a recent study has indicated that the motor deficit must reside elsewhere since rescuing cerebellar volume and cellularity with a SHH agonist does not improve motor function or motor learning in Ts65Dn [28]. SHH signaling has also been implicated in oligodendrocyte specification and differentiation [22, 71]. Changes in cell proliferation, SHH signaling, and Olig2 expression have all been shown to affect DS brain development. Therefore, we reasoned that the SC, known for its dependence both on SHH signaling and Olig2 expression for patterning and cell type specification, may be a primary site of motor dysfunction in DS.

During neural tube development, gradients of Bone Morphogenetic Protein and SHH arise from the roof and floor plates, respectively, to direct dorsoventral patterning [20, 58]. These gradients establish 7 dorsal and 5 ventral progenitor domains within the ventricular zone (VZ) surrounding the central canal [65, 73]. As development proceeds, dorsal progenitors give rise to sensory afferents and local INs within the dorsal horn of the SC [65]. SHH-responsive ventral progenitors, however, give rise to motor neurons and several classes of local INs within the ventral horn (VH). One of these ventral SC progenitor domains expresses OLIG2 and is known as the pMN domain. The pMN domain arises in the ventral neural tube of developing embryos and contains bipotential precursor cells that can differentiate into either motor neurons (MNs) or oligodendrocytes (OLs) [2, 46]. Upon differentiation, MNs migrate away from the midline into the gray matter of the VH, where they form local networks with INs and also send long-range, topographically ordered projections to muscles. While OLs also originate in the ventral SC, they migrate through several streams to form distinct SC white matter tracts. During development, OLIG2 selectively heterodimerizes with the basic helix-loop-helix transcription factor NEUROG2 to prompt MN differentiation and then later with the homeobox domain transcription factor NKX2.2 to promote oligodendrogenesis [37, 46, 63, 76]. Thus, these three transcription factors form a complex, temporally regulated switch to control the designation and proper allocation of MNs and OLs. Furthermore, due to cross-repressive signals that define strict boundaries between progenitor domains [11], studies show that alterations in the expression of OLIG2 can impact fates of cells arising from the immediately adjacent progenitor domains marked by the NKX2.2 and IRX3 transcription factors [43]. These adjacent domains give rise to several classes of ventral INs [2].

Here, we analyze the progenitor domains and the principal spinal neuronal and glial cells they produce in the well-characterized Ts65Dn mouse model of DS [53, 54, 60]. Ts65Dn mice have an extra freely segregating marker chromosome containing roughly 100 triplicated mouse chromosome 16 (Mmu16) genes that are syntenic to Hsa21 genes, including Olig2 [19]. In addition, these mice display motor changes that are similar to those seen in people with DS [15, 29, 30, 53, 60]. We measured the size and behavior of neural progenitor domains starting at embryonic day (E)10.5 and determined the number and position of their postmitotic progeny at various time points over the lifespan. Our work identifies early prenatal changes in the progenitor populations that give rise to MNs, INs, and OLs, as well as perturbations in these populations that arise postnatally. These changes are observed at both the gene expression and cellular levels and are concomitant with deficits in attainment of developmental milestones in pups as well as motor reflexes and strength in adult mice. Taken together, our data identify multiple cellular changes in the SC and point to this motor control center as a potential source of the motor deficits in Ts65Dn animals and people with DS.



All murine experiments were conducted according to international ethical standards and approved by the Institutional Animal Care and Use Committees (IACUC) of Boston University. Animals were housed in cages with standard bedding and a nestlet square. Rodent chow and water were available ad libitum. The colony was maintained on a 12:12 light/dark cycle, with lights on at 7:00 AM.

B6EiC3Sn.BLiA-Ts(1716)65Dn/DnJ (Ts65Dn; stock number 005252) mice were purchased from The Jackson Laboratory (Bar Harbor, ME). Ts65Dn female mice were bred with B6EiC3Sn.BLiAF1/J (F1 hybrid; stock number 003647) males. Studies were performed at embryonic days (E)10.5, 12.5, and E14.5, postnatal days (P)30 and 60, and at 10-11 months. All experiments were conducted on tissue collected from a colony established in 2012 and maintained until 2014.

Tissue collection

Embryonic spinal cord collection

Breeding pairs were established so that vaginal plugs could be checked twice daily. The presence of a vaginal plug was designated as E0.5. A 10% weight gain at E10 was used to confirm pregnancy [35]. Male and female embryos were collected and processed for fluorescent immunohistochemical staining or for gene expression analyses.

For embryonic immunohistochemical studies, embryos were extracted, heads and viscera were rapidly removed, and the remaining tissue was fixed for 1–24 h in 4% paraformaldehyde (PFA) at 4 °C. Fixation time depended on age of embryo. Fixed tissue was then washed three times in 1x phosphate-buffered saline (PBS), placed in 30% sucrose for 16-24 h at 4 °C, and embedded in optimal cutting temperature compound (OCT; Sakura, Torrance, CA). Embedded tissue was frozen rapidly and either stored at − 80 °C or immediately sectioned into 16-μm thick frozen sections using a cryostat (ThermoFisher Scientific, Waltham, MA). Whole-body serial coronal sections were taken along the body’s rostro-caudal axis, and mounted on Superfrost® Plus slides (Fisher Scientific, Waltham, MA). Slides were dried at room temperature then stored at − 80 °C.

For embryonic gene expression analysis, embryos were extracted and decapitated in ice-cold DEPC-treated 1x PBS. Embryonic SCs were rapidly removed from the developing spinal column and snap frozen in liquid nitrogen before storage at − 80 °C. Prior to dissections, all surfaces and tools were treated with an anti-RNase solution, RNaseZap (ThermoFisher Scientific, Waltham, MA).

Adult tissue collection

For postnatal immunohistochemical studies, male mice were anesthetized with a xylazine/ketamine cocktail and were transcardially perfused with 4% PFA in 1x PBS. SCs were extracted and post-fixed for 16 h in 4% PFA at 4 °C and then sunk in 30% sucrose overnight. SCs were then dissected into cervical, thoracic, lumbar, and sacral segments. These subsections were embedded in OCT (Sakura, Torrance, CA), frozen, and stored at − 80 °C.

For adult gene expression studies, male mice were anesthetized with 2.5% isoflurane in a 3/7 O2/N2O mixture and euthanized by decapitation. SCs were removed from the spinal column, placed into ice-cold DEPC-treated 1 x PBS, then dissected into cervical, thoracic, lumbar, and sacral segments. SC subsections were then snap frozen in liquid nitrogen and stored at − 80 °C. Similar to the embryonic spinal cord collection, prior to dissections, all surfaces and tools were treated with RNaseZap (ThermoFisher Scientific, Waltham, MA).

Genotyping and sex determination

Embryonic limb buds or adult tail samples were taken from each animal at the time of collection and digested overnight at 55 °C with Proteinase K (Denville Scientific, Holliston, MA). DNA was then purified and extracted using standard phenol/chloroform extraction methods (Fisher Bioreagents).

Genotyping and sex determination were performed by polymerase chain reaction (PCR) using specific primers for theTs65Dn translocation breakpoints on Mmu16 and Mmu17, and the sex-determining region of the Y chromosome (SRY). To confirm the accuracy of the translocation-based genotyping, genotyping was occasionally also carried out by quantitative (q) PCR using specific primers for the amyloid precursor protein (App) gene, which is triplicated in Ts65Dn mice, and ApoB, which is not triplicated in these mice (Table 1) [41, 55]. Relative quantities of these two genes were compared, and animals that showed a 1.5-fold expression in App compared to ApoB were designated as trisomic.

Table 1 Primer sequences for genotyping of embryonic and adult mice and sex-determination of embryonic mice

Gene expression studies

For gene expression studies, total RNA was isolated from the SCs using Trizol® following the manufacturer’s instructions (Thermo Fisher Scientific, MA). Genomic DNA was first removed using DNase Treatment and Removal Kit (Ambion). Purified RNA was quantified then reverse-transcribed into cDNA using high-capacity cDNA reverse transcription kit per manufacturer’s instructions (Thermo Fisher Scientific, MA). qRT-PCR was then carried out using SYBR® Green reagents (Thermo Fisher Scientific, MA) and validated QuantiTect® exon-spanning primers for genes of interest (Qiagen, GER) (primer sequences listed in Additional file 1: Table S1). Trisomic and euploid samples from the same cohort were analyzed side by side to avoid batch errors. All values were first normalized to the housekeeping gene GAPDH, then presented as a relative quantity of euploid samples. Three to six mice from each genotypic group were used and data are shown as mean ± SE. A Student’s t test was used to assess significance at p < 0.05.


When necessary, depending on the antigen and tissue-penetrance of the primary antibody, antigen retrieval was performed by microwaving slides in 10 mM sodium citrate buffer for 1 min at maximum power, followed by 10 min at minimum power or by incubating in a 70 °C water-bath for 35 min in a 1:10 solution of HistoVT One® (Nacalai Tesque, Kyoto, Japan). Slides were then washed three times in 1x PBS for 5 min each and incubated in a blocking solution comprised of 5% normal donkey or normal goat serum, 0.2% Triton® X-100, and 1x PBS for 1 h at room temperature. This was followed by incubation in primary antibody overnight at room temperature. Slides were washed 3 times in 1x PBS and incubated with fluorescent secondary antibodies in blocking solution for 1 h at room temperature. Finally, slides were mounted in Vectashield with DAPI (Vector Laboratories). The following primary antibodies were used: rabbit anti-Oligodendrocyte Transcription Factor 2 (1:300, Millipore, AB9610), rabbit anti-Parvalbumin (1:1000, Swant, PV25), rabbit anti-Calretinin (1:1000, Swant, 769913), rabbit anti-Calbindin (1:1000, Swant, D-28 k), mouse anti-Hb9 (1:10, DSHB, 81.5c10-s), rabbit anti-Islet 1 (1:300, Abcam, AB20670), goat anti-Choline Acetyltransferase (1:50, Millipore, AB144p), mouse anti-PAX6 (1:50, DSHB), mouse anti-NKX2.2 (1:50, DSHB) mouse anti-NKX6.1 (1:50, DSHB), mouse anti-CC1/APC (1:500, Calbiochem, OP80), Guinea pig anti-NG2 (1:2000, gift from Dr. William Stallcup), CASPR and NF186 (gifts from Dr. Manzoor Bhat, used according to previously published methods [48]), and mouse anti-CASPR (NIH NeuroMab, 75-001). The following secondary antibodies were used (AlexaFluor, 1:250 dilution, Thermo Fisher Scientific): donkey anti-rabbit 555 (A31572), donkey anti-goat 488 (A11055), donkey anti-mouse 488 (A21202), goat anti-rabbit 546 (A11035), goat anti-rabbit 488 (A11008), goat anti-Guinea pig 546 (A11074), and goat anti-rat 488 (A11006). Different immunohistochemistry (IHC) protocols were used to optimize detection of target proteins. See Additional file 1: Table S2 for specific antibody information.

Confocal microscopy and cell counting

For all markers used, three to four sections per animal were imaged using a Zeiss LSM 710 confocal microscope system (Carl Zeiss, GER). Sixteen 1-μm thick z-stacks (1024x1024 resolution) of each region of interest (ROI) were acquired using a 20X objective (N.A = 0.8). For some embryonic sections, tiled images were necessary in order to capture the entire bilateral ventral horn ROI within each SC section. After imaging, labeled cells were then either automatically counted using Volocity (Improvision) software following manual validation of randomly selected samples or manually counted using ImageJ and LSM Image Browser software. In postnatal tissue, analysis was limited to the ventral portion (as determined by bisecting the central canal), dorsal corticospinal tract (DCST), and lateral funiculus (LF) of the lumbar spinal cord. In embryonic tissue, only the ventral portion of the caudal SC was imaged and analyzed. All ROIs across all ages and genotypes were chosen to encapsulate the entire anatomical region of interest, removing the need for any random stereological sampling.

Data analysis

Cell counts from the ventral horn were processed first by image, then by animal (two images were taken from each animal), and finally by genotype. All cell density counts were normalized to a 100 μm3 ROI unless otherwise noted. These density measurements corresponded to cell density within the identified ROI and served to standardize measurements across animals, ages, and genotypes when the size of the area of interest varied. For example, this normalization was necessary when comparing cell populations across ages or when the size of the ventral SC varied slightly from animal to animal. When no standardization was needed, cell number was reported. Outliers in data sets from both euploid and trismic mice were statistically determined using a calculation of interquartile range (IQR). All data points outside of the IQR fences were excluded from analysis without bias. In general, zero to two outliers were identified in each data set. All variables were assessed with a two-tailed, independent samples Student’s t test, and passed both the Shapiro-Wilks normality test and an equal variance test, unless otherwise noted. Additional statistical tests, such as two-factor ANOVAs, are noted where applicable.

Behavioral studies

Motor developmental milestones and motor coordination and strength were assessed using the hind-limb reflex task and the hanging wire task as previously described [48]. All experiments were conducted in the light phase between 10:00 AM and 1:00 PM. All behavioral tests were performed blindly without prior knowledge of genotype. Care was taken to minimize animal stress by allowing a standard period of habituation to the testing room each day prior to the start of testing. Additionally, spatial and olfactory cues were minimized by utilizing the same area of testing and cleaning with ethanol after each use by an animal. Four to eight mice per genotype were used.


Embryonic analyses

Immunohistochemical analysis of spinal neural and glial populations at E10.5

To identify the MN progenitors within the OLIG2+ pMN domain of the caudal/lumber SC, we began our embryonic SC analysis at E10.5 (Fig. 1A), when MNs and INs progenitors are still actively proliferating and before oligodendrogenesis has started (Calver et al. 1998). First, all OLIG2+ progenitors were counted at E10.5 in both Ts65Dn (n = 6) and euploid (n = 6) mice. There was a 64.8% ± 22.8% significant increase in the density of OLIG2+ cells in the trisomic embryos compared to the euploid controls (Fig. 1B; p < 0.05). The OLIG2+ domain was also significantly wider, dorso-ventrally, in the Ts65Dn SC (Fig. 1C; p < 0.05). In contrast to these changes in OLIG2+ cells, we found no significant change in numbers of ISL1, NKX2.2, or NKX6.1-expressing cells at E10.5 (Fig. 1B).

Fig. 1
figure 1

Cellular populations at E10.5 in the Ts65Dn spinal cord. A A representative confocal image of a cross section of an E10.5 spinal cord from a euploid mice stained for Isl1, OLIG2, NKX6.1, and NKX2.2. A′ An inset showing a magnified view of the OLIG2 progenitor domain in euploid and Ts65Dn spinal cords. B Average cell density of trisomic animals compared to euploid controls. Trisomic animals show a significant increase of Olig2+ pMN progenitor cells as well as a trend towards an increase in the number of fated motor neurons (Olig2+/Isl1+) and oligodendrocyte precursor cells (OPCs) (Olig2+/Nkx2.2+). C Along with an increase in Olig2+ density, the width of the Olig2+ pMN domain is significantly increased. D We also assessed changes in proliferation of the progenitors between genotypes and found E no difference in PH3+ cells in total or changes in their distribution measured F laterally from the lumen or G from the ventral edge (n = 6 euploid and 6 Ts65Dn; *p < 0.05, #p < 0.2)

At this developmental time point, OLIG2+/ISL1+ cells are fated to differentiate into postmitotic MNs. A non-significant increase in this population was observed in Ts65Dn mice (139% ± 22%) compared to euploid littermates (100% ± 14.5%) (Fig. 1B; p = 0.17). Also, at E10.5, co-expression of OLIG2 and NKX2.2 indicates a transition of MN progenitors to OL progenitor cells (OPCs). The number of OPCs was substantially increased in Ts65Dn mice (179% ± 33.9%) compared to euploid littermates (100% ± 6.8%) but did not reach statistically significant levels (Fig. 1B, p = 0.067). The proportion of MN progenitors and OPCs of all OLIG2+ cells was the same between genotypes, indicating that the increase in OLIG2+ cells affects both subpopulations (MN and OPCs) equally in Ts65Dn SC (data not shown).

Lastly, we used the mitotic marker phospho-histone H3 (pH 3) to label actively proliferating cells in the ventral SC. We found no change in the number of pH 3+ cells by genotype (Fig. 1E), nor did we detect differences in pH 3+ cell location with respect to the neural tube lumen (Fig. 1D, F) or in their dorsoventral distribution (Fig. 1D, G).

Gene expression analysis of spinal neural and glial populations at E12.5

We used qRT-PCR to measure the expression of genes associated with spinal MNs, OLs, and INs. At E12.5, we measured a significant 1.5-fold increase in expression of Olig2 and a significant increase in expression of Hb9, another gene also expressed by MN progenitors, in trisomic mice (n = 3) compared to euploid littermates (n = 3) (Fig. 2D, p < 0.05). No change was observed in expression of Irx3, a transcription factor expressed in all INs arising in progenitor domains dorsal to the pMN (data not shown; p = 0.2). Similarly, no changes were observed in levels of Nkx2.2 or Sim1, transcription factors expressed by IN progenitors in the domain ventral to the pMN (Fig. 2D). These findings indicate that changes in the pMN domain of trisomic animals did not affect gene expression in neighboring domains at this age.

Fig. 2
figure 2

Expression and population analyses at E12.5 in the Ts65Dn spinal cord. A Representative confocal images of cross sections of an E12.5 spinal cord stained for Isl1, Olig2, Pax6, B Nkx2.2, and C Nkx6.1. A′ An inset showing a comparison of OLIG2, ISL1, and PAX6 staining in euploid and Ts65Dn spinal cords. D qRT-PCR analysis shows a significant increase in expression levels of Hb9 and Olig2 in the trisomic spinal cords (n = 3 euploid and 3 Ts65Dn; *p < 0.05). E At E12.5, there is no significant difference in the number of Olig2+ cells or in F the size of the various progenitor domains between euploid and trisomic individuals. G Trisomic animals show a significant increase in the number of Isl1+ migrating motor neurons as well as a significant increase in the number of abventricular Pax6+ inhibitory interneurons and Nkx2.2+ excitatory interneurons (n = 4 euploid and 5 Ts65Dn; *p < 0.05, **p < 0.01, ***p < 0.001)

Analysis of spinal neural and glial populations at E12.5

In order to correlate these gene expression findings with cellular development, we measured the density and distribution of ventral OLs, MNs, and INs in the SC at E12.5 by triple immunostaining for three population-specific transcription factors, OLIG2, ISL1, and PAX6 in Ts65Dn embryos (n = 5) and their euploid littermates (n = 4) (Fig. 2A). Based on previous studies (Calver et al., 1998), all OLIG2+/ISL1- progenitors at this developmental stage are fated to the OL lineage and all ISL1+ cells are OLIG2- postmitotic MNs. As expected, since MN production peaks around E9 and ceases by E12 [40, 43], all OLIG2+ cells were in fact ISL1- at this developmental time point. We used PAX6 as a pan-IN marker for all inhibitory ventral INs (i.e., V0, V1, and V2 INs) [2]. To determine if expansion of the OLIG2 domain in Ts65Dn at E10.5 has an effect on NKX2.2+ V3 excitatory INs 2 days later, we also stained for NKX2.2 and NKX6.1 (Fig. 2B, C), two transcription factors expressed by this subclass of ventral INs [46, 61, 64]. Importantly, because NKX6.1 can also be expressed in a small group of ISL1+ MNs, cells immunopositive for both of these markers were excluded from counts in order to restrict the NKX6.1 counts to the IN population only.

Oligodendrocyte lineage at E12.5

In contrast to measurements at E10.5, we found no changes in the overall OLIG2+ cell density in Ts65Dn mice compared to their euploid littermates. Further subdivision of the OLIG2+ population into two groups—one containing cells within the pMN domain near the midline and another abventricular group of cells migrating away from the ventricular zone—showed no significant change in the ventricular OLIG2+ cells (Fig. 2A, E). The length of the OLIG2+ pMN domain was also not different from controls (Fig. 2F, p = 0.15). Taking these trends into consideration, the pMN domain abnormalities found at E10.5 were seen to have diminished two days later.

Motor neurons at E12.5

The total ISL1+ cell population (combined cohort of migrating cells and postmitotic MNs) showed a large but non-significant increase in Ts65Dn mice (127.8% ± 4.66%) compared to their euploid littermates (100% ± 12.2%) (p = .077). When further broken down into two cohorts, migrating ISL1+ cells and terminally differentiated MNs within the dorsal columns, the postmitotic MN population was not changed but the density of the migrating ISL1+ cells was significantly increased in trisomic animals (212.7% ± 12.9%) compared to euploid littermates (100% ± 2%) (Fig. 2G; p < .001).

Interneurons at E12.5

Significant increases in migrating INs were detected in the Ts65Dn SC at E12.5. The total PAX6+ IN population (combined cohort of ventricular and abventricular cells) was significantly increased in Ts65Dn mice (146.9% ± 11.48%) compared to euploid littermates (100% ± 8.2%) (p = .016) and this was due to large increases in the abventricular PAX6+ cell group in Ts65Dn (163.5% ± 10.3%) vs. euploid littermates (100% ± 8.1%) (Fig. 2G; p = 0.012). In addition, while we found no change in the ventricular NKX2.2+ population, there was a significant increase in the abventricular NKX2.2+ population in Ts65Dn mice (118% ± 3.5%) compared to euploid controls (100% ± 0.9%) (Fig. 2G; p < 0.01). Concordant with the normal numbers of ventricular cells, the length of the NKX2.2+ progenitor domain was not significantly changed (Fig. 2F). The numbers of NKX6.1+ cells and the length of the progenitor domain marked by NKX6.1 expression were also unchanged compared to controls (Fig. 2F, G).

Analysis of spinal neural and glial populations at E14.5

To determine whether gene expression changes measured at E12.5 persist at E14.5, we measured expression levels of Olig2, Hb9, Nkx2.2, Sim1, and Irx3 using qRT-PCR. We found no significant change in Ts65Dn (n = 7) SC compared to euploid controls (n = 5) (Fig. 3c). To quantify the number and distribution of OLs, MNs, and INs in the SC at E14.5, we stained for OLIG2, NKX2.2, NKX6.1, and ISL1 in Ts65Dn mice (n = 6) and their euploid littermates (n = 7) (Fig. 3a, b). At this developmental timepoint, all OLIG2+ cells are ISL1-, indicating an OL fate restriction, while NKX2.2 marks the V3 IN lineage and NKX6.1+ cells represent the V1, V2, and V3 IN lineages [2]. Since NKX6.1 can still be co-expressed within a group of ISL1+ MNs, these double-positive cells were excluded from counts in order to restrict the NKX6.1 counts to IN populations only. Lastly, ISL1 marks MNs that are at this point fully clustered into terminal MN columns (Fig. 3a). Similar to the gene expression results, we found no significant differences in the density of all examined MNs, INs or OLs at E14.5 (Fig. 3d).

Fig. 3
figure 3

Expression and population analyses at E14.5 in the Ts65Dn spinal cord. a Representative confocal images of cross sections of an E14.5 spinal cord stained for a Isl1, Olig2, b Nkx2.2, Nkx6.1, and Olig2. At E14.5, there are c no changes in gene expression measured by qRT-PCR (n = 5 euploid and 7 Ts65Dn) or d changes in the cell density of OPCs, motor neurons, or interneurons (n = 7 euploid and 6 Ts65Dn)

Postnatal analyses

To continue the characterization of spinal MNs, OLs, and INs, we quantified the subsets of postmitotic cells that arise from the OLIG2+ pMN progenitor domain as well as from the directly adjacent progenitor domains marked by NKX2.2 and IRX3 expression. As in our embryonic analyses, we limited our focus to the ventral portion of the lumbar SC to specifically analyze neuronal populations that participate in central pattern generators (CPGs) and produce motor output related to locomotion. We also sampled an ascending and a descending white matter tract, the lateral funiculus (LF) and dorsocorticospinal tract (DCST), respectively, to analyze OL maturation and white matter organization within the lumbar SC.

Changes in motor and interneuron populations

Because HB9 and ISL1 expression change over the life span, we utilized a functional marker related to MN neurotransmitter synthesis, choline acetyltransferase (ChAT), to quantify the number of cholinergic MNs in adult SC. At postnatal day 60 (P60), immunohistochemical staining of ChAT in the VH of the lumbar cord identified no changes in cell number between euploid (n = 4) and Ts65Dn mice (n = 4) (Fig. 4c, f). Similarly, we used expression of calcium-binding proteins to identify postmitotic inhibitory INs in the ventral SC. No change was seen in either parvalbumin (PV) or calbindin (CB) immunoreactive ventral INs (Fig. 4a, b, f). However, there was a significant increase in the number of Calretinin (CR) positive interneurons in the Ts65Dn mice, with a 63.6 ± 14.5% increase over the euploid controls (Fig. 4d, f; p < 0.05).

Fig. 4
figure 4

Postnatal motor neuron and interneuron analyses. Representative confocal images of the ventral horn of lumbar sections in the P60 spinal cord from both euploid and Ts65n mice, stained for a acetyl choline transferase (ChAT), b calbindin (CB), c parvalbumin (PV), and d calretinin (CR). e At P60, qRT-PCR gene expression analysis shows a significant increase in expression level of Hb9 and a significant decrease in the expression of Irx3 in the trisomic spinal cords (n = 3 euploid and 3 Ts65Dn; *p < 0.05). f At P60, there is a significant increase in the number of CR+ cells in the trisomic animals (n = 4 euploid and 4 Ts65Dn; *p < 0.05) while at g 10–11 months of age, there are significantly fewer ChAT+ motor neurons and CB+ interneurons in the trisomic animals (n = 4 euploid and 6 Ts65Dn, *p < 0.05)

At P60, gene expression analysis showed a 2.0 ± 0.5-fold increase in relative gene expression of Hb9 in Ts65Dn whole SC (n = 3) compared to euploid controls (n = 3) (Fig. 4e; p < 0.05). Hb9 expression is a hallmark of embryonic postmitotic MNs and is essential for their differentiation, consolidation, and columnar specification. Hb9 expression is thought to be transient and ectopic expression of format has been shown to impact the development of spinal INs [68]. Thus, the fact that Hb9 gene expression is increased in trisomic mice during development and adulthood may indicate a defect in transcriptional programs governing either pathfinding or maturation of these neurons or neighboring INs. In fact, at this time, Irx3 expression in Ts65Dn SC (n = 3) was decreased to 0.58 ± 0.04-fold relative expression compared to euploid littermates (n = 3) (Fig. 4e; p < 0.05). No change was observed in Chat, Parv, Calb, or Calr gene expression in these mice (Fig. 4e).

Notably, while there was no significant change in number of MNs within the VH at P60, by 10–11 months of age, there were significantly fewer ChAT+ MNs in trisomic mice (n = 6) compared to euploid littermates (n = 4) (Fig. 4g; p = 0.018). This suggests a degenerative MN phenotype and supports a recent report that described MN degeneration both in humans with DS and the Tc1 mouse model of DS [72]. By 10–11 months, the number of CB+ INs in the VH of the trisomic SC (n = 6) was also significantly decreased compared to euploid controls (n = 4) (Fig. 4g; p < 0.05). Previous work has shown that CB specifically marks a subset of V1 INs known as Renshaw cells [7, 9]. These cells are known to participate in local networks that lead to recurrent inhibition loops with MNs [45, 56]. The concomitant decrease in both cell populations in the aged Ts65Dn SCs suggests that at least two cell types forming the CPGs in the SC are defective. In addition to these significant decreases at 10–11 months, we show that there is no difference in number of CR+ INs at this age (Fig. 4g). This finding is in contrast to the significant increase in number of CR+ cells found in the trisomic animals at P60, indicating that CR immunoreactive interneurons are likely being lost during aging in the trisomic animals as well. In contrast, PV immunoreactive ventral INs were found in normal numbers in the Ts65Dn SC (Fig. 4g).

Changes in oligodendrocyte populations

Due to the major contribution of OLIG2 to the differentiation and maturation of OLs, and recent work highlighting OL maturation and white matter defects in Ts65Dn brains and in post-mortem brains from individuals with DS [47], we assessed OL maturation and white matter properties in Ts65Dn SCs. Using OLIG2 as a marker of all OLs, we quantified the OLIG2+/CC1+/NG2- mature OL population and the OLIG2+/CC1-/NG2+ immature OL population in the descending DSCT and the ascending LF in Ts65Dn SCs and euploid controls. In the DCST, the overall number of OLIG2+ OLs did not differ between Ts65Dn mice (n = 3 at P30, n = 4 at P60) and euploid littermates (n = 3 at P30, n = 4 at P60). However, at P30 there was a 16.3% ± 8% decrease (p < 0.05) and at P60 there was a 4.1% ± 1.6% decrease (p < 0.05) in mature OLs in Ts65Dn mice compared to euploid controls (Fig. 5a, c, e). At both ages, this decrease in mature OLs was coincident with an increase in immature OLs. In 10–11 months old animals, the maturational profile of OLs in the DSCT was similar to euploid samples, but at this age we found a significant overall reduction of OLIG2+ cells (30.3% ± 6.6%) compared to euploid controls (Fig. 5g; p < 0.05).

Fig. 5
figure 5

Oligodendrocyte maturation analyses in the DCST and LF. Representative confocal images of the a dorsal corticospinal tract (DCST) and b lateral funiculus (LF) stained with Olig2+ to mark all oligodendrocyte lineage cells and CC1+ and Ng2+ to mark mature and immature oligodendrocytes, respectively. In the DCST at c P30 and e P60, there is a significantly smaller percentage of mature CC1+ oligodendrocytes in the trisomic animals. g By 10–11 months, this change in maturation is no longer present, but there are significantly fewer oligodendrocytes in total in the trisomic animals. d, f, h In the LF at all ages analyzed, there is a significantly higher percentage of CC1+ mature oligodendrocytes in the trisomic animals (P30 n = 3 euploid and 3 Ts65Dn; P60 n = 4 euploid and 4 Ts65Dn; 10–11 months n = 4 euploid and 6 Ts65Dn; *p < 0.05)

Interestingly, we found a markedly different profile of OL maturation in the ascending LF. At P30, P60, and 10–11 months, there were more CC1+ mature OLs in the trisomic animals compared to euploid controls. Specifically, at P30, there was a significant increase of 6.5 ± 1.3% in mature OLs, while at P60 there was a significant increase of 3.3% ± 1.1% in mature OLs, and at 10–11 months there was a significant increase of 5.7% ± 2.0% in mature OLs in Ts65Dn mice compared to euploid controls (Fig. 5d, f, h; p < 0.05). Unlike in the DCST, we found no decrease in total OL number in the LF of trisomic animals with age.

To determine whether the reductions in nodes of Ranvier found previously in forebrain white matter tracts were also present in the SC [47], we immunostained for the nodal proteins CASPR and Neurofascin (NF186). In the DCST at P30, there was a significant decrease in nodes of Ranvier in Ts65Dn mice (n = 3) compared to euploid controls (n = 3), but not at P60 or at 10–11 months (Fig. 6a, b; p<0.05). The same profile was found in the LF (Fig. 6c; p < 0.05). Assessment of Caspr and Nfsc (Neurofascin) gene expression during white matter development at P7 and P15, and after the peak of white matter development at P60, showed large but non-significant decreases in relative expression of both genes in Ts65Dn mice (Fig. 6d).

Fig. 6
figure 6

Analysis of the nodes of Ranvier in the DCST and LF. a A representative confocal image of the nodes of Ranvier stained with the nodal marker NF186+ and the paranodal marker CASPR+ in the DCST. b, c In both the DCST and LF, there are significantly fewer nodes of Ranvier in the trisomic animals at P30. This difference is not present at P60 or at 10–11 months in either the DCST or LF (P30 n = 3 euploid and 3 Ts65Dn; P60 n = 4 euploid and 4 Ts65Dn; 10-11 months n = 4 euploid and 6 Ts65Dn; *p < 0.05). d qRT-PCR analysis of Nfasc and Caspr gene expression in the spinal cord shows no significant difference between euploid and trisomic at P7, P15, or P60 (P7 n = 5 euploid and 2 Ts65Dn; P15 n = 3 euploid and 3 Ts65Dn; P60 n = 3 euploid and 3 Ts65Dn)

Longitudinal behavioral analyses

Since widespread and temporally dynamic changes were observed in Ts65Dn MNs, INs and OLs during development and in adulthood, we reanalyzed our previously published data to identify indices of motor function. Developmental milestone data showed that P3-P21 Ts65Dn male pups mice performed worse on several motor-based tasks compared to euploid littermates [5, 47, 48]. In particular, Ts65Dn pups showed a delay in achieving the following tasks: surface righting, cliff aversion, and negative geotaxis (Table 2). In addition, as adults, these Ts65Dn male mice performed worse on the hanging wire task, a strength test that engages several motor control systems within the CNS, and on the hind-limb reflex test, which is a reflexive behavior that is largely independent of cortical motor control (Fig. 7; data previously shown in [48]).

Table 2 Motor developmental milestones
Fig. 7
figure 7

Motor abnormalities in Ts65Dn. Motor function assessed by a–d hind-limb extension reflex and e hanging wire tests of 3-month-old euploid and Ts65Dn mice show significant impairment in Ts65Dn mice. For the hind-limb extension reflex, each mouse was suspended by its tail for 10 s and its hind-limb posture was scored as 2 (a), 1 (b), or 0 (c). For the hanging wire test, each mouse is placed on top of a standard wire cage and the latency to fall from the lid is recorded when the lid is turned upside down. Score values shown in d and e represent mean ± SEM of 6 tests on three different days and 2 tests on two different days, respectively (n = 14 euploid, 15 Ts65Dn; **p < 0.0001, *p < 0.05)


In this study, we examined the effect of trisomy on OLs, MNs, and INs in the SC of the Ts65Dn mouse model of DS. Overall, there were multiple perturbations in neuronal and glial cell populations both embryonically and postnatally. The prenatal studies identified an increase in the size of the OLIG2+ pMN domain leading to transient increases in the number of committed MNs, OPCs, and INs from neighboring progenitor domains. Additionally, following these changes in early development, we found maturation and degeneration phenotypes affecting these cell classes in the adult SC. While some populations were affected only transiently during development, longer-lasting effects on these cells could be measured during adulthood and into aging. Based on the timing and the cell types affected, the data are consistent with a developmental disturbance at least partly caused by Olig2 triplication, confirming the essential role of this transcription factor in proper patterning and development of ventral neurons and glia in the SC [46].

Embryonically, MNs exhibited changes in their progenitor number and in the size of their progenitor domain in trisomic mice at E10.5. These early disturbances were followed by an increase in the production of migrating ISL1+ MNs that continued longer than controls and was still present at E12.5. We also found an altered distribution of OLs and INs within the VH at E12.5, perhaps related to the overexpression of Olig2 and the shifts in pMN domain size and MN production. The number of PAX6+ INs found still migrating in the ventral SC was significantly increased at E12.5, a time when all ventral spinal INs would have normally reached their final destination [24, 50]. The consistent increase in the number of abventricular INs (also seen in the NKX2.2+ population) and MNs indicates altered development of the excitatory/inhibitory neurons within the growing SC in Ts65Dn mice. This is consistent with previous findings showing an over-production of inhibitory INs in the developing cortex of Ts65Dn mice [10].

Interestingly, Olig2 expression is known to affect cell proliferation and cell cycle exit in the pMN [37], and its overexpression has been shown to increase the size of the pMN at early embryonic timepoints and to maintain progenitor cells in a proliferative state [46, 61], delaying their maturation. This scenario appears to be occurring during Ts65Dn development. For example, the increased number of OLIG2+ cells (and a trend towards an increase in OLIG2+/ISL1+ MN progenitors and the OLIG2+/NKX2.2+ IN progenitors) at E10.5, and the succeeding increase in Olig2 and Hb9 gene expression at E12.5, are correlated with an increase in ISL1+, PAX6+, and NKX2.2+ migrating (i.e., non-terminally differentiated) progenitors. Thus, we posit that Olig2 triplication may be affecting the cell cycle exit, migration, or differentiation properties of ventral spinal neurons. More cellular analyses are needed to identify the specific etiology underlying these changes.

Despite these alterations during early SC development, by E14.5, there were no detectable differences in cell number in the Ts65Dn samples. Nevertheless, it is likely that the early, transient disturbance in cell production and allocation leads to improper cell arrival times, affecting subsequent circuit formation. This altered development may contribute to the delayed developmental milestone acquisition seen in both perinatal Ts65Dn pups and infants with DS. For example, the CPGs that drive stereotyped locomotor behavior are dependent on proper wiring and firing of all classes of ventral interneurons. Within the CPG circuit, each subclass of INs governs a specific modular aspect of locomotion by directly or indirectly innervating MNs [26, 33, 34, 39]. Delayed arrival of MNs and INs into these circuits or improper synaptic integration may significantly impact motor output [33, 36, 75]. In addition, spinal INs can form long-range as well as local connections [3] and, therefore, may impact larger areas of motor control.

Our data also show neuronal and glial perturbations in the adult Ts65Dn SC, some of which are exacerbated with age. For example, although at P60 there are no changes in ChAT+ MNs and an increase in ventral IN populations expressing CR, by 10–11 months numbers of ChAT+ cells and CB+ INs are decreased in Ts65Dn SCs while there is no change in CR cell numbers. The differences in numbers of cells could reflect gene expression changes, may be due to neurodegeneration or to changes in target muscles as muscular abnormalities have been observed in older Ts65Dn mice [12]. This loss of MNs late in life also replicates the decrease in MNs reported in both the Tc1 mouse model of DS and in tissue derived from people with DS [72].

Similar to findings in the Ts65Dn cerebral cortex and in the brains of people with DS [47], we found changes in OL maturation in the SC. However, there is surprising variability in OL maturation between ascending and descending axonal tracts and this difference correlates with the respective source of each OL population. For example, in the DCST, which is comprised of dorsally derived OLs [69], there is a decrease in mature OLs at both P30 and P60, and by 10–11 months there is a reduced number of OLIG2+ cells. In contrast, in the LF, populated by ventrally derived OLs, there are more mature OLs in the trisomic animals at all ages examined and the size of the OLIG2+ population appears normal. The correlation between the OL maturation state and their dorsoventral source may provide some clues as to the origin of the defect. In the SC, dorsal OLs can be generated independently of SHH [8, 23], while the ventral OLs are derived from a progenitor domain that is specified by the SHH gradient emanating from the notochord and floorplate. It is interesting to note that SHH signaling has also been implicated in the development of cerebellar hypoplasia in DS. Together, these findings may identify SHH signaling as a major contributor to motor delays in DS. While SHH agonist (SAG) treatment at birth corrected the cerebellar growth deficit in Ts65Dn animals [28], it did not improve motor function. Our data indicate that SAG may impact OL fate commitment and maturation if supplied at earlier developmental time points. Taken together with our previous studies, these results suggest that OL maturation is altered throughout the Ts65Dn CNS and that the magnitude of this effect varies across different regions of the SC.


Overall, our data uncover cellular and molecular alterations in the SC that occur during development and postnatal life in the Ts65Dn mouse model of DS. This study identifies several regions and cell types within the SC that may be potential targets for improving CNS development and general health outcomes in people with DS.

The significant effects on MNs and IN cell types have wide implications for the organization of locomotor CPGs in the cord and may be directly linked to the gait, fine motor control and muscle tone abnormalities seen in people with DS. The dynamic changes uncovered in our study correlate well with clinical observations in infants, adolescents, and adults with DS who present with hypotonia and areflexia at birth and delays in achieving motor developmental milestones in infancy, but eventually compensate for such deficits later in life.

Moreover, OL dysfunction in the SC mimics OL changes previously observed in brains of people with DS and in Ts65Dn mice, pointing to a CNS-wide defect. Hypomyelination in people with DS may be a systems-level anatomical alteration, driven either by the gene dosage imbalance of Olig2 (and Olig1), decreased sensitivity to SHH, or a combination of the two. Our previous work and current study suggest that these myelination defects could potentially underlie both the cognitive and motor changes seen in people with DS and present a targetable mechanism for drug development.

Availability of data and materials

Not applicable


  1. Akshoomoff NA, Courchesne E, Press GA, Iragui V. Contribution of the cerebellum to neuropsychological functioning: evidence from a case of cerebellar degenerative disorder. Neuropsychologia. 1992;30(4):315–28.

    PubMed  CAS  Google Scholar 

  2. Alaynick WA, Jessell TM, Pfaff SL. SnapShot: spinal cord development. Cell. 2011;146(1):178–178.e171.

    PubMed  PubMed Central  CAS  Google Scholar 

  3. Arber S. Motor circuits in action: specification, connectivity, and function. Neuron. 2012;74(6):975–89.

    PubMed  CAS  Google Scholar 

  4. Aylward EH, Habbak R, Warren AC, Pulsifer MB, Barta PE, Jerram M, Pearlson GD. Cerebellar volume in adults with Down syndrome. Arch Neurol. 1997;54(2):209–12.

    PubMed  CAS  Google Scholar 

  5. Aziz NM, Guedj F, Pennings JLA, Olmos-Serrano JL, Siegel A, Haydar TF, Bianchi DW. Lifespan analysis of brain development, gene expression and behavioral phenotypes in the Ts1Cje, Ts65Dn and Dp(16)1/Yey mouse models of Down syndrome. Dis Model Mech. 2018.

  6. Belichenko PV, Kleschevnikov AM, Salehi A, Epstein CJ, Mobley WC. Synaptic and cognitive abnormalities in mouse models of Down syndrome: exploring genotype-phenotype relationships. J Comp Neurol. 2007;504(4):329–45.

    PubMed  CAS  Google Scholar 

  7. Benito-Gonzalez A, Alvarez FJ. Renshaw cells and Ia inhibitory interneurons are generated at different times from p1 progenitors and differentiate shortly after exiting the cell cycle. J Neurosci. 2012;32(4):1156–70.

    PubMed  PubMed Central  CAS  Google Scholar 

  8. Cai J, Qi Y, Hu X, Tan M, Liu Z, Zhang J, Li Q, Sander M, Qiu M. Generation of oligodendrocyte precursor cells from mouse dorsal spinal cord independent of Nkx6 regulation and Shh signaling. Neuron. 2005;45(1):41–53.

    PubMed  CAS  Google Scholar 

  9. Carr PA, Alvarez FJ, Leman EA, Fyffe RE. Calbindin D28k expression in immunohistochemically identified Renshaw cells. Neuroreport. 1998;9(11):2657–61.

    PubMed  CAS  Google Scholar 

  10. Chakrabarti L, Best TK, Cramer NP, Carney RS, Isaac JT, Galdzicki Z, Haydar TF. Olig1 and Olig2 triplication causes developmental brain defects in Down syndrome. Nat Neurosci. 2010;13(8):927–34.

    PubMed  PubMed Central  CAS  Google Scholar 

  11. Chen JA, Huang YP, Mazzoni EO, Tan GC, Zavadil J, Wichterle H. Mir-17-3p controls spinal neural progenitor patterning by regulating Olig2/Irx3 cross-repressive loop. Neuron. 2011;69(4):721–35.

    PubMed  PubMed Central  CAS  Google Scholar 

  12. Cisterna B, Costanzo M, Scherini E, Zancanaro C, Malatesta M. Ultrastructural features of skeletal muscle in adult and aging Ts65Dn mice, a murine model of Down syndrome. Muscles Ligaments Tendons J. 2013;3(4):287–94.

    PubMed  Google Scholar 

  13. Cole KJ, Abbs JH, Turner GS. Deficits in the production of grip forces in Down syndrome. Dev Med Child Neurol. 1988;30(6):752–8.

    PubMed  CAS  Google Scholar 

  14. Contestabile, A., T. Fila, C. Ceccarelli, P. Bonasoni, L. Bonapace, D. Santini, R. Bartesaghi and E. Ciani. Cell cycle alteration and decreased cell proliferation in the hippocampal dentate gyrus and in the neocortical germinal matrix of fetuses with down syndrome and in Ts65Dn mice. Hippocampus. 2007

  15. Costa AC, Walsh K, Davisson MT. Motor dysfunction in a mouse model for Down syndrome. Physiol Behav. 1999;68(1-2):211–20.

    PubMed  CAS  Google Scholar 

  16. Das I, Park JM, Shin JH, Jeon SK, Lorenzi H, Linden DJ, Worley PF, Reeves RH. Hedgehog agonist therapy corrects structural and cognitive deficits in a Down syndrome mouse model. Sci Transl Med. 2013;5(201):201ra120.

    PubMed  PubMed Central  Google Scholar 

  17. de Graaf G, Buckley F, Skotko BG. Estimates of the live births, natural losses, and elective terminations with Down syndrome in the United States. Am J Med Genet A. 2015;167A(4):756–67.

    PubMed  Google Scholar 

  18. Desmond JE, Gabrieli JD, Wagner AD, Ginier BL, Glover GH. Lobular patterns of cerebellar activation in verbal working-memory and finger-tapping tasks as revealed by functional MRI. J Neurosci. 1997;17(24):9675–85.

    PubMed  PubMed Central  CAS  Google Scholar 

  19. Duchon A, Raveau M, Chevalier C, Nalesso V, Sharp AJ, Herault Y. Identification of the translocation breakpoints in the Ts65Dn and Ts1Cje mouse lines: relevance for modeling Down syndrome. Mamm Genome. 2011;22(11-12):674–84.

    PubMed  PubMed Central  CAS  Google Scholar 

  20. Ericson J, Muhr J, Jessell TM, Edlund T. Sonic hedgehog: a common signal for ventral patterning along the rostrocaudal axis of the neural tube. Int J Dev Biol. 1995;39(5):809–16.

    PubMed  CAS  Google Scholar 

  21. Fabbro F, Tavano A, Corti S, Bresolin N, De Fabritiis P, Borgatti R. Long-term neuropsychological deficits after cerebellar infarctions in two young adult twins. Neuropsychologia. 2004;42(4):536–45.

    PubMed  CAS  Google Scholar 

  22. Ferent J, Zimmer C, Durbec P, Ruat M, Traiffort E. Sonic Hedgehog signaling is a positive oligodendrocyte regulator during demyelination. J Neurosci. 2013;33(5):1759–72.

    PubMed  PubMed Central  CAS  Google Scholar 

  23. Fogarty M, Richardson WD, Kessaris N. A subset of oligodendrocytes generated from radial glia in the dorsal spinal cord. Development. 2005;132(8):1951–9.

    PubMed  CAS  Google Scholar 

  24. Francius C, Harris A, Rucchin V, Hendricks TJ, Stam FJ, Barber M, Kurek D, Grosveld FG, Pierani A, Goulding M, Clotman F. Identification of multiple subsets of ventral interneurons and differential distribution along the rostrocaudal axis of the developing spinal cord. PLoS One. 2013;8(8):e70325.

    PubMed  PubMed Central  CAS  Google Scholar 

  25. Goodliffe JW, Olmos-Serrano JL, Aziz NM, Pennings JL, Guedj F, Bianchi DW, Haydar TF. Absence of Prenatal Forebrain Defects in the Dp(16)1Yey/+ Mouse Model of Down Syndrome. J Neurosci. 2016;36(10):2926–44.

    PubMed  PubMed Central  CAS  Google Scholar 

  26. Gosgnach S. The role of genetically-defined interneurons in generating the mammalian locomotor rhythm. Integr Comp Biol. 2011;51(6):903–12.

    PubMed  Google Scholar 

  27. Guidi S, Ciani E, Bonasoni P, Santini D, Bartesaghi R. Widespread proliferation impairment and hypocellularity in the cerebellum of fetuses with down syndrome. Brain Pathol. 2011;21(4):361–73.

    PubMed  Google Scholar 

  28. Gutierrez-Castellanos N, Winkelman BH, Tolosa-Rodriguez L, Devenney B, Reeves RH, De Zeeuw CI. Size does not always matter: Ts65Dn Down syndrome mice show cerebellum-dependent motor learning deficits that cannot be rescued by postnatal SAG treatment. J Neurosci. 2013;33(39):15408–13.

    PubMed  PubMed Central  CAS  Google Scholar 

  29. Hampton TG, Stasko MR, Kale A, Amende I, Costa AC. Gait dynamics in trisomic mice: quantitative neurological traits of Down syndrome. Physiol Behav. 2004;82(2-3):381–9.

    PubMed  CAS  Google Scholar 

  30. Haydar TF, Reeves RH. Trisomy 21 and early brain development. Trends Neurosci. 2012;35(2):81–91.

    PubMed  CAS  Google Scholar 

  31. Henderson SE, Morris J, Frith U. The motor deficit in Down's syndrome children: a problem of timing? J Child Psychol Psychiatry. 1981;22(3):233–45.

    PubMed  CAS  Google Scholar 

  32. Hernandez-Gonzalez S, Ballestin R, Lopez-Hidalgo R, Gilabert-Juan J, Blasco-Ibanez JM, Crespo C, Nacher J, Varea E. Altered distribution of hippocampal interneurons in the murine Down Syndrome model Ts65Dn. Neurochem Res. 2015;40(1):151–64.

    PubMed  CAS  Google Scholar 

  33. Hinckley CA, Alaynick WA, Gallarda BW, Hayashi M, Hilde KL, Driscoll SP, Dekker JD, Tucker HO, Sharpee TO, Pfaff SL. Spinal locomotor circuits develop using hierarchical rules based on motorneuron position and identity. Neuron. 2015;87(5):1008–21.

    PubMed  PubMed Central  CAS  Google Scholar 

  34. Hinckley CA, Pfaff SL. Imaging spinal neuron ensembles active during locomotion with genetically encoded calcium indicators. Ann N Y Acad Sci. 2013;1279:71–9.

    PubMed  PubMed Central  CAS  Google Scholar 

  35. Johnson KL, Tao K, Stroh H, Kallenbach L, Peter I, Richey L, Rust D, Bianchi DW. Increased fetal cell trafficking in murine lung following complete pregnancy loss from exposure to lipopolysaccharide. Fertil Steril. 2010;93(5):1718–1721.e1712.

    PubMed  CAS  Google Scholar 

  36. Lanuza GM, Gosgnach S, Pierani A, Jessell TM, Goulding M. Genetic identification of spinal interneurons that coordinate left-right locomotor activity necessary for walking movements. Neuron. 2004;42(3):375–86.

    PubMed  CAS  Google Scholar 

  37. Lee SK, Lee B, Ruiz EC, Pfaff SL. Olig2 and Ngn2 function in opposition to modulate gene expression in motor neuron progenitor cells. Genes Dev. 2005;19(2):282–94.

    PubMed  PubMed Central  CAS  Google Scholar 

  38. Lejeune J, Turpin R, Gautier M. Mongolism; a chromosomal disease (trisomy). Bull Acad Natl Med. 1959;143(11-12):256–65.

    PubMed  CAS  Google Scholar 

  39. Levine AJ, Lewallen KA, Pfaff SL. Spatial organization of cortical and spinal neurons controlling motor behavior. Curr Opin Neurobiol. 2012;22(5):812–21.

    PubMed  PubMed Central  Google Scholar 

  40. Li H, de Faria JP, Andrew P, Nitarska J, Richardson WD. Phosphorylation regulates OLIG2 cofactor choice and the motor neuron-oligodendrocyte fate switch. Neuron. 2011;69(5):918–29.

    PubMed  PubMed Central  CAS  Google Scholar 

  41. Liu DP, Schmidt C, Billings T, Davisson MT. Quantitative PCR genotyping assay for the Ts65Dn mouse model of Down syndrome. Biotechniques. 2003;35(6):1170–4 1176, 1178 passim.

    PubMed  CAS  Google Scholar 

  42. Mai CT, Isenburg J, Langlois PH, Alverson CJ, Gilboa SM, Rickard R, Canfield MA, Anjohrin SB, Lupo PJ, Jackson DR, Stallings EB, Scheuerle AE, Kirby RS. Population-based birth defects data in the United States, 2008 to 2012: Presentation of state-specific data and descriptive brief on variability of prevalence. Birth Defects Res A Clin Mol Teratol. 2015;103(11):972–93.

    PubMed  PubMed Central  CAS  Google Scholar 

  43. Meijer DH, Kane MF, Mehta S, Liu H, Harrington E, Taylor CM, Stiles CD, Rowitch DH. Separated at birth? The functional and molecular divergence of OLIG1 and OLIG2. Nat Rev Neurosci. 2012;13(12):819–31.

    PubMed  PubMed Central  CAS  Google Scholar 

  44. Melyn MA, White DT. Mental and developmental milestones of noninstitutionalized Down's syndrome children. Pediatrics. 1973;52(4):542–5.

    PubMed  CAS  Google Scholar 

  45. Moore NJ, Bhumbra GS, Foster JD, Beato M. Synaptic Connectivity between Renshaw Cells and Motoneurons in the Recurrent Inhibitory Circuit of the Spinal Cord. J Neurosci. 2015;35(40):13673–86.

    PubMed  PubMed Central  CAS  Google Scholar 

  46. Novitch BG, Chen AI, Jessell TM. Coordinate regulation of motor neuron subtype identity and pan-neuronal properties by the bHLH repressor Olig2. Neuron. 2001;31(5):773–89.

    PubMed  CAS  Google Scholar 

  47. Olmos-Serrano JL, Kang HJ, Tyler WA, Silbereis JC, Cheng F, Zhu Y, Pletikos M, Jankovic-Rapan L, Cramer NP, Galdzicki Z, Goodliffe J, Peters A, Sethares C, Delalle I, Golden JA, Haydar TF, Sestan N. Down Syndrome Developmental Brain Transcriptome Reveals Defective Oligodendrocyte Differentiation and Myelination. Neuron. 2016a;89(6):1208–22.

    PubMed  PubMed Central  CAS  Google Scholar 

  48. Olmos-Serrano JL, Tyler WA, Cabral HJ, Haydar TF. Longitudinal measures of cognition in the Ts65Dn mouse: Refining windows and defining modalities for therapeutic intervention in Down syndrome. Exp Neurol. 2016b;279:40–56.

    PubMed  PubMed Central  Google Scholar 

  49. Palisano RJ, Walter SD, Russell DJ, Rosenbaum PL, Gemus M, Galuppi BE, Cunningham L. Gross motor function of children with down syndrome: creation of motor growth curves. Arch Phys Med Rehabil. 2001;82(4):494–500.

    PubMed  CAS  Google Scholar 

  50. Panayiotou E, Panayi E, Lapathitis G, Francius C, Clotman F, Kessaris N, Richardson WD, Malas S. Pax6 is expressed in subsets of V0 and V2 interneurons in the ventral spinal cord in mice. Gene Expr Patterns. 2013;13(8):328–34.

    PubMed  CAS  Google Scholar 

  51. Pereira K, Basso RP, Lindquist AR, da Silva LG, Tudella E. Infants with Down syndrome: percentage and age for acquisition of gross motor skills. Res Dev Disabil. 2013;34(3):894–901.

    PubMed  Google Scholar 

  52. Pinter JD, Eliez S, Schmitt JE, Capone GT, Reiss AL. Neuroanatomy of Down's syndrome: a high-resolution MRI study. Am J Psychiatry. 2001;158(10):1659–65.

    PubMed  CAS  Google Scholar 

  53. Rachidi M, Lopes C. Mental retardation and associated neurological dysfunctions in Down syndrome: a consequence of dysregulation in critical chromosome 21 genes and associated molecular pathways. Eur J Paediatr Neurol. 2008;12(3):168–82.

    PubMed  Google Scholar 

  54. Reeves RH, Irving NG, Moran TH, Wohn A, Kitt C, Sisodia SS, Schmidt C, Bronson RT, Davisson MT. A mouse model for Down syndrome exhibits learning and behaviour deficits. Nat Genet. 1995;11(2):177–84.

    PubMed  CAS  Google Scholar 

  55. Reinholdt LG, Ding Y, Gilbert GJ, Czechanski A, Solzak JP, Roper RJ, Johnson MT, Donahue LR, Lutz C, Davisson MT. Molecular characterization of the translocation breakpoints in the Down syndrome mouse model Ts65Dn. Mamm Genome. 2011;22(11-12):685–91.

    PubMed  PubMed Central  CAS  Google Scholar 

  56. Renshaw B. Central effects of centripetal impulses in axons of spinal ventral roots. J Neurophysiol. 1946;9:191–204.

    PubMed  CAS  Google Scholar 

  57. Rigoldi C, Galli M, Albertini G. Gait development during lifespan in subjects with Down syndrome. Res Dev Disabil. 2011;32(1):158–63.

    PubMed  Google Scholar 

  58. Roelink H, Porter JA, Chiang C, Tanabe Y, Chang DT, Beachy PA, Jessell TM. Floor plate and motor neuron induction by different concentrations of the amino-terminal cleavage product of sonic hedgehog autoproteolysis. Cell. 1995;81(3):445–55.

    PubMed  CAS  Google Scholar 

  59. Roper RJ, Baxter LL, Saran NG, Klinedinst DK, Beachy PA, Reeves RH. Defective cerebellar response to mitogenic Hedgehog signaling in Down [corrected] syndrome mice. Proc Natl Acad Sci U S A. 2006;103(5):1452–6.

    PubMed  PubMed Central  CAS  Google Scholar 

  60. Rueda N, Florez J, Martinez-Cue C. Mouse models of Down syndrome as a tool to unravel the causes of mental disabilities. Neural Plast. 2012;2012:584071.

    PubMed  PubMed Central  Google Scholar 

  61. Sander M, Paydar S, Ericson J, Briscoe J, Berber E, German M, Jessell TM, Rubenstein JL. Ventral neural patterning by Nkx homeobox genes: Nkx6.1 controls somatic motor neuron and ventral interneuron fates. Genes Dev. 2000;14(17):2134–9.

    PubMed  PubMed Central  CAS  Google Scholar 

  62. Siarey RJ, Stoll J, Rapoport SI, Galdzicki Z. Altered long-term potentiation in the young and old Ts65Dn mouse, a model for Down Syndrome. Neuropharmacology. 1997;36(11-12):1549–54.

    PubMed  CAS  Google Scholar 

  63. Sun T, Dong H, Wu L, Kane M, Rowitch DH, Stiles CD. Cross-repressive interaction of the Olig2 and Nkx2.2 transcription factors in developing neural tube associated with formation of a specific physical complex. J Neurosci. 2003;23(29):9547–56.

    PubMed  PubMed Central  CAS  Google Scholar 

  64. Sun T, Echelard Y, Lu R, Yuk DI, Kaing S, Stiles CD, Rowitch DH. Olig bHLH proteins interact with homeodomain proteins to regulate cell fate acquisition in progenitors of the ventral neural tube. Curr Biol. 2001;11(18):1413–20.

    PubMed  CAS  Google Scholar 

  65. Tanabe Y, Jessell TM. Diversity and pattern in the developing spinal cord. Science. 1996;274(5290):1115–23.

    PubMed  CAS  Google Scholar 

  66. Tatsumi K, Isonishi A, Yamasaki M, Kawabe Y, Morita-Takemura S, Nakahara K, Terada Y, Shinjo T, Okuda H, Tanaka T, Wanaka A. Olig2-Lineage Astrocytes: A Distinct Subtype of Astrocytes That Differs from GFAP Astrocytes. Front Neuroanat. 2018;12:8.

    PubMed  PubMed Central  Google Scholar 

  67. Tavano A, Grasso R, Gagliardi C, Triulzi F, Bresolin N, Fabbro F, Borgatti R. Disorders of cognitive and affective development in cerebellar malformations. Brain. 2007;130(Pt 10):2646–60.

    PubMed  Google Scholar 

  68. Thaler J, Harrison K, Sharma K, Lettieri K, Kehrl J, Pfaff SL. Active suppression of interneuron programs within developing motor neurons revealed by analysis of homeodomain factor HB9. Neuron. 1999;23(4):675–87.

    PubMed  CAS  Google Scholar 

  69. Tripathi RB, Clarke LE, Burzomato V, Kessaris N, Anderson PN, Attwell D, Richardson WD. Dorsally and ventrally derived oligodendrocytes have similar electrical properties but myelinate preferred tracts. J Neurosci. 2011;31(18):6809–19.

    PubMed  PubMed Central  CAS  Google Scholar 

  70. Vicari S. Motor development and neuropsychological patterns in persons with Down syndrome. Behav Genet. 2006;36(3):355–64.

    PubMed  Google Scholar 

  71. Wang LC, Almazan G. Role of Sonic Hedgehog Signaling in Oligodendrocyte Differentiation. Neurochem Res. 2016;41(12):3289–99.

    PubMed  CAS  Google Scholar 

  72. Watson-Scales S, Kalmar B, Lana-Elola E, Gibbins D, La Russa F, Wiseman F, Williamson M, Saccon R, Slender A, Olerinyova A, Mahmood R, Nye E, Cater H, Wells S, Yu YE, Bennett DLH, Greensmith L, Fisher EMC, Tybulewicz VLJ. Analysis of motor dysfunction in Down Syndrome reveals motor neuron degeneration. PLoS Genet. 2018;14(5):e1007383.

    PubMed  PubMed Central  Google Scholar 

  73. Wine-Lee L, Ahn KJ, Richardson RD, Mishina Y, Lyons KM, Crenshaw EB 3rd. Signaling through BMP type 1 receptors is required for development of interneuron cell types in the dorsal spinal cord. Development. 2004;131(21):5393–403.

    PubMed  CAS  Google Scholar 

  74. Yu T, Li Z, Jia Z, Clapcote SJ, Liu C, Li S, Asrar S, Pao A, Chen R, Fan N, Carattini-Rivera S, Bechard AR, Spring S, Henkelman RM, Stoica G, Matsui S, Nowak NJ, Roder JC, Chen C, Bradley A, Yu YE. A mouse model of Down syndrome trisomic for all human chromosome 21 syntenic regions. Hum Mol Genet. 2010;19(14):2780–91.

    PubMed  PubMed Central  CAS  Google Scholar 

  75. Zhang Y, Narayan S, Geiman E, Lanuza GM, Velasquez T, Shanks B, Akay T, Dyck J, Pearson K, Gosgnach S, Fan CM, Goulding M. V3 spinal neurons establish a robust and balanced locomotor rhythm during walking. Neuron. 2008;60(1):84–96.

    PubMed  PubMed Central  CAS  Google Scholar 

  76. Zhou Q, Choi G, Anderson DJ. The bHLH transcription factor Olig2 promotes oligodendrocyte differentiation in collaboration with Nkx2.2. Neuron. 2001;31(5):791–807.

    PubMed  CAS  Google Scholar 

Download references


We would like to thank Cristina Pineda and Amber Pasion for their work maintaining and genotyping the Ts65Dn animals and Liam McCarthy for measurements of Caspase-3 staining.


Funded by NIH grants NS095340, NS076503 and U54HD090257.

Author information

Authors and Affiliations



NMA conceived of the project, conducted postnatal experiments, helped to write the manuscript, and managed MRB who conducted the prenatal experiments and edited the manuscript. JAK conducted postnatal experiments and helped to write and edit the manuscript. JLOS conducted the behavioral experiments and edited the manuscript. TFH managed the project, constructed the figures, and wrote and edited the manuscript. VG edited and performed final review of the manuscript. All authors read and approved the final manuscript.

Corresponding author

Correspondence to Tarik F. Haydar.

Ethics declarations

Ethics approval and consent to participate

This work was conducted in accordance with Boston University Institutional Biosafety and Animal Care and Use approvals.

Consent for publication

All authors consent to publication.

Competing interests

The authors declare no competing interest. Jose Luis Olmos Serrano is now an employee of Biogen. This work was completed before he joined the company. Biogen did not have a role in the design, conduct, analysis, interpretation, or funding of the research related to this work.

Additional information

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Additional file 1: Table S1.

Primers used for qRT-PCR. Table S2. Antibody information for immunohistochemistry. Extended Immunohistochemistry Conditions.

Rights and permissions

Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (, which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver ( applies to the data made available in this article, unless otherwise stated.

Reprints and permissions

About this article

Check for updates. Verify currency and authenticity via CrossMark

Cite this article

Aziz, N.M., Klein, J.A., Brady, M.R. et al. Spatiotemporal development of spinal neuronal and glial populations in the Ts65Dn mouse model of Down syndrome. J Neurodevelop Disord 11, 35 (2019).

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI: