Search tips
Search criteria 


Logo of jneurosciThis ArticleAbout the JournalFor AuthorsSign up for AlertsThe Journal of NeuroscienceSociety for Neuroscience
J Neurosci. 2012 March 14; 32(11): 3818–3829.
PMCID: PMC3679185

Motor Neuron Rescue in Spinal Muscular Atrophy Mice Demonstrates That Sensory-Motor Defects Are a Consequence, Not a Cause, of Motor Neuron Dysfunction


The loss of motor neurons (MNs) is a hallmark of the neuromuscular disease spinal muscular atrophy (SMA); however, it is unclear whether this phenotype autonomously originates within the MN. To address this question, we developed an inducible mouse model of severe SMA that has perinatal lethality, decreased motor function, motor unit pathology, and hyperexcitable MNs. Using an Hb9-Cre allele, we increased Smn levels autonomously within MNs and demonstrate that MN rescue significantly improves all phenotypes and pathologies commonly described in SMA mice. MN rescue also corrects hyperexcitability in SMA motor neurons and prevents sensory-motor synaptic stripping. Survival in MN-rescued SMA mice is extended by only 5 d, due in part to failed autonomic innervation of the heart. Collectively, this work demonstrates that the SMA phenotype autonomously originates in MNs and that sensory-motor synapse loss is a consequence, not a cause, of MN dysfunction.


The survival motor neuron 1 (SMN1) gene encodes a protein that is essential for spliceosome assembly (Schrank et al., 1997; Pellizzoni et al., 1998). While complete loss of SMN is lethal to all cells, low levels of SMN cause the neuromuscular disease spinal muscular atrophy (SMA) (Lefebvre et al., 1995; Crawford and Pardo, 1996; Coovert et al., 1997; Lefebvre et al., 1997). The pathology of SMA is paradoxical because SMN is ubiquitously expressed in all cells, yet motor neurons (MNs) preferentially degenerate.

SMA has been modeled in several organisms to address SMN′s cellular requirements. In zebrafish and Caenorhabditis elegans, restoring SMN in MNs rescues neuromuscular junction (NMJ) pathology, while in Drosophila, both MN and muscle rescue are required to correct pathology (Chang et al., 2008; Boon et al., 2009; Briese et al., 2009). Survival analysis in these models is complicated, since they rely on either maternal transcripts or temporally discordant drivers to accomplish SMN rescue.

Conflicting evidence exists regarding whether neuromuscular dysfunction in SMA mice originates in MNs. Gavrilina et al. (2008) demonstrated that CNS-specific SMN restoration rescued the phenotype of a severe SMA mouse model, albeit with leaky expression in skeletal muscle. Importantly, muscle specific rescue where there was no leakiness in the CNS had no survival benefit.

In contrast, mice with disease-relevant levels of SMN only within MNs and oligodendrocytes do not develop severe SMA, as one would expect from a cell-autonomous disease, but instead develop an adult form of SMA (Park et al., 2010). This suggests an additive involvement of muscle, Schwann cells, and/or peripheral factors in defining disease severity. Alternatively, these results could be due to inefficient Olig2-Cre-mediated recombination, or an unknown disease modifying role of Olig2+ oligodendrocytes (Park et al., 2010). To date, genetic experiments in mice have failed to exclusively target motor neurons, making it difficult to draw conclusions pertaining to MN-autonomous disease mechanisms.

An important recent finding is that a loss of the central synapses, particularly the proprioceptive inputs onto MN somata and proximal dendrites, both parallels and precedes the pattern of MN loss in SMA mice (Ling et al., 2010; Park et al., 2010; Mentis et al., 2011). Mechanistically, this could indicate that defects within afferent neurons play a causative role in disease that is external to the MN (Mentis et al., 2011). If true, a simplistic interpretation would be that MNs are not affected by low Smn levels and would not benefit from autonomously increased Smn dosage; rather MNs are relatively healthy cells, whose dysfunction and loss is attributed to aberrant synaptic input.

Here, we directly address the question of MN specificity by generating a Cre-inducible mouse model of severe SMA. Using an Hb9-Cre allele, we demonstrate that MN rescue dramatically improves all neuromuscular phenotypes and pathologies observed in severe SMA model mice; however, survival is only extended 5 d due in part to failed autonomic innervation of the heart. This work demonstrates that the neuromuscular phenotype in SMA mice autonomously originates in MNs, while their lethality is multifactorial.

Materials and Methods

Ethics statement.

All studies performed on mice were in accordance with the Institutional Animal Care and Use Committee regulations in place at Children's Memorial Research Center and Northwestern University's Animal Care and Use Committee guidelines, and were specifically approved under Protocols 2006-22 and 2008-03.

Animal models.

Animals were kept in a controlled vivarium at 25°C and 50% humidity with a 12 h light/dark photoperiod and monitored for health. The official strain designations for the alleles used in this manuscript are as follows: SMN2, FVB.Cg-Tg(SMN2)89Ahmb Smntm1Msd; Smn2B-Neo, B6.127-Smn1tm1Cdid; Smn2B, B6.127-Smn1tm1.1Cdid; Hb9-Cre, B6;129S-Hlxb9tm4(cre)Tmj; ZGFP, B6.Cg-Tg(ACTB-Bgeo/GFP)21Lbe (Arber et al., 1999; Monani et al., 2000; Novak et al., 2000; Hammond et al., 2010). The official name for the severe inducible model reported here [(SMN2)89Ahmb+/−, Smn2B-Neo/2B-Neo] is Tg(SMN2)89Ahmb/J, Smn1tm1Cdid/ tm1Cdid.

Severe inducible SMA pups were generated by crossing a breeder stock of SMN2+/+; Smn2B-Neo/+ SMA mice with a Smn2B-Neo/+ mouse to create SMN2+/−; Smn2B-Neo/2B-Neo SMA pups. For MN-rescue experiments, an Hb9-Cre+/− mouse was intercrossed with a Smn2B-Neo/+ heterozygote. F1 progeny that were positive for both the Smn2B-Neo and the Hb9-Cre alleles were backcrossed to the SMN2+/−; Smn2B-Neo/+ breeder stock to create SMA mice containing both with (MN-rescued SMA) and without (severe inducible SMA) Hb9-Cre. In all of the described experiments, both male and female pups were used in proportions approximated to be equal.


The presence of the neomycin cassette was verified via PCR using a forward primer within neomycin (5′-gcattaaagcttggctggac) and a reverse primer in Smn intron 7 (5′-gagaccgaggcaggctaac) that amplifies a neomycin specific band of 353 bp (Smn2B-Neo). The addition of a third primer within intron 6 (5′-tcccaggcagttttagactca) allows for the detection of a WT band of 750bp (Smn+). When the neomycin cassette has been removed by Cre-recombinase, a third 850 bp band corresponds to the excised allele (Smn2B). The presence of the Hb9-Cre allele was detected using generic Cre primers (forward, 5′-atgtccaatttactgaccg; reverse, 5′-cgccgcataaccagtgaaac). Assessment of the (SMN2)89Ahmb allele was conducted as described previously (Gavrilina et al., 2008).


In all phenotypic assays, the researcher recording the score was blinded to the genotype of the litter being assessed. Tube test was conducted as described by Heier et al. (2010a). Righting reflex was monitored on odd days beginning at postnatal day 3 (P3) and defined as the time taken to turn over and place all four paws simultaneously on a hard benchtop after being placed in supine position. If righting did not occur in, 1 min the test was scored as a failure. Electrocardiography (ECG) was conducted as described by Heier et al. (2010b). The end stage was defined as 2 consecutive days of weight loss and an inability to right within 60 s in cage bedding.

Western blot analysis.

To quantify Smn levels, 5 μg of total protein per tissue was resolved on a NuPage Novex 4–12% Bis-Tris gel and transferred to nitrocellulose membrane. Smn was detected by Western blot using the Li-COR Odyssey system as described previously (Hammond et al., 2010).


NMJ staining was performed on whole-mount intercostals (ICs) and triangularis sterni (TS) using a combination of neurofilament [1:100; 2H3; Developmental Hybridoma Bank (DHB)], synaptic vesicle 2 (SV2; 1:10; DHB), and rhodamine conjugated α-bungarotoxin (αBTX; 1:250; Invitrogen). Briefly, whole-mount tissues were dissected and fixed in 2% paraformaldehyde overnight at 4°C. The following day, they were washed in PBS for 2 h at room temperature (RT). Primary antibodies (NF and SV2) were then added in blocking buffer (5% bovine serum, 2% Triton X-100, 0.5% glycine in PBT). Samples were incubated in primary for 48–72 h at RT on a rocker, washed three times for 10 min each in PBS, and incubated in secondary antibody (1:250, GAM-488 and 594-αBTX) for 24 h at RT. Samples were again washed three times for 10 min each in PBS and mounted on slides with Clear Mount mounting media (Invitrogen).

For MN staining, spinal cords were dissected, fixed in 2% PFA at 4°C overnight, cryoprotected in 30% sucrose for 12–24 h, and embedded in OCT. Serial sections (12 μm thick) were collected, and to avoid repeat counts, every 15th section (180 μm apart) was used to quantify MN number. Before ChAT and Islet-1/2 staining, one slide per series was stained with fluorescent Nissl (0.5 mg/ml cresyl violet) to assist in determining the exact location within the spinal cord. Following antigen retrieval, equivalent sections from an adjacent slide were stained in 5% donkey serum for ChAT (Millipore Bioscience Research Reagents; 1:100) and Islet-1/2 (DHB; 4D5, 1:100 plus 2H3, 1:100). Only double-positive cells localized in the ventral horn were classified as MNs. Tyrosine hydroxylase (TH), vesicular glutamate transporter 1 (vGlut1), and Smn staining, as well as Smn gem counts were conducted as described previously (DiDonato et al., 2003; Heier et al., 2010a; Ling et al., 2010; Park et al., 2010; Le et al., 2011).

NMJ innervation/maturity quantification.

All NMJs were imaged whole mount on a Leica spinning disc confocal microscope using Slidebook software. Z stacks were deconvolved in Slidebook, and the projection image was used for final analysis. Images were de-identified and randomized before quantification for blinding purposes. Blinded images were assessed for innervation and maturity using Adobe Photoshop, CS4 extended edition. Innervation status was defined visually as fully innervated (>80%), partially innervated (15–80%), or denervated (≤15%). Postsynaptic maturity was defined as junctions containing homogeneous plaques, folds, perforations, or secondary structure. Only after quantification was complete were the images reidentified for statistical analysis.


Mice at P4–P5 were deeply anesthetized with isofluorane, decapitated, and eviscerated. The spinal cord was quickly removed and embedded in 2.5% w/v agar, and super glued to a stainless-steel platform, and 350 μm transverse slices were made using a Leica 1000 vibratome as described previously (Quinlan et al., 2011). During both spinal cord isolation and slicing, the spinal cord was immersed in 1–4°C high-osmolarity dissecting solution containing the following (in mm): 234 sucrose, 2.5 KCl, 0.1 CaCl2 · 2H2O, 4 MgSO4 · 7H2O, 15 HEPES, 11 glucose, and 1 Na2PO4, pH 7.4 when bubbled with 95% O2/5% CO2. After cutting, the slices were incubated for >1 h at 30°C in incubating solution containing the following (in mm): 126 NaCl, 2.5 KCl, 2 CaCl2 · 2H2O, 2 MgCl2 · 6H2O, 26 NaHCO3, and 10 glucose, pH 7.4 when bubbled with 95% O2/5% CO2. During recording, slices were perfused at a rate of 2.5–3.0 ml/min with a modified Ringer's solution containing the following (in mm): 111 NaCl, 3.09 KCl, 25 NaHCO3, 1.10 KH2PO4, 1.26 MgSO4, 2.52 CaCl2, and 11.1 glucose. Whole-cell patch-clamp recording was performed using 1–4 MΩ glass electrodes containing the following (in mm): 150 Texan red dextran (3000 molecular weight; Invitrogen), 138 K-gluconate, 10 HEPES, 5 ATP-Mg, and 0.3 GTP-Li (all from Sigma). Electrodes were positioned using a Sutter Instrument MP-285 motorized micromanipulator. Whole-cell patch-clamp measurements were performed at room temperature using the Multiclamp 700B amplifier (Molecular Devices).

Only neurons maintaining a resting potential of −50 mV or lower, an action potential height of >0 mV, a series resistance of ≤25 MΩ, and an input resistance of ≤200 MΩ were included in this study. Recordings were performed in current- and voltage-clamp modes [more details available in the study by Quinlan et al. (2011)]. In voltage-clamp mode, holding potential was set to −90 mV, and neurons were subjected to a slow, depolarizing voltage ramp of 12 mV/s, bringing the cell to +6 mV in 8 s, and then back to the holding potential in the following 8 s. Persistent inward current (PIC) amplitudes were measured from leak-subtracted current traces. In current-clamp mode, depolarizing ramps were used for testing ION (the current level at firing onset), IOFF (the current level at cessation of firing), and the frequency–current relationship. Characteristics of the action potential, including overshoot (past 0 mV), duration at half peak, and rate of rise were measured from the first spike elicited from the current ramp. Threshold voltage was determined as the voltage at which the rate of rise of the membrane potential exceeded 10 mV/ms, indicating the beginning of the spike. Synaptic potentials were quantified as the number of sharp deflections in membrane potential (either depolarizing or hyperpolarizing) occurring over 5–10 s. Data was collected on Winfluor software (University of Strathclyde, Glasgow, Scotland) and analyzed using Spike2 software (Cambridge Electronic Design). Z stacks were obtained using a Bio-Rad 2100 MPD laser scanning microscope. The Coherent Chameleon Ultra II laser was used at 920 nm. Bio-Rad LaserSharp software was used to collect 1024 × 1024 pixel Z stacks, up to 200 μm depth, in 1.0 μm steps, and using a Kalman 4 filter. Image analysis was performed using ImageJ (NIH).

Statistical analysis.

Statistical analysis was analyzed using Graph Pad Prism software (version 4.0) and Microsoft Excel. Kaplan–Meier survival curves were compared using log-rank tests. Significance in weights, tube test scores, innervation status, and postsynaptic maturity was determined using either a one- or two-way ANOVA with a Bonferroni post hoc comparison or Student's t test as appropriate. Significance pertaining to MN counts and heart rate was analyzed with a Student's t test.


Smn inducible model of severe SMA

Smn inducible SMA mice were generated by breeding the Smn1tm1Cdid allele (hereafter referred to as Smn2B-Neo) with the commonly used Tg(SMN2)89Ahmb allele (hereafter referred to as SMN2) (Monani et al., 2000; Hammond et al., 2010). Smn2B-Neo/2B-Neo embryos die by E9 due to low Smn protein levels (1–3%), but Smn dosage can be dramatically increased if the floxed neomycin cassette is removed by Cre-recombinase [discussed extensively in the study by Hammond et al. (2010)]. By breeding one copy of the SMN2 transgene to a Smn2B-Neo/2B-Neo background (SMN2+/−; Smn2B-Neo/2B-Neo), we increased Smn levels to 6% relative to SMN2+/+; Smn+/+ controls (Fig. 1A). Importantly, this rescued the lethality observed in Smn2B-Neo/2B-Neo embryos and allowed for postnatal survival.

Figure 1.
Phenotypic characterization of severe inducible SMA mice. A, Western blot analysis of Smn levels. The homozygous presence of the neomycin cassette decreases Smn to 6% relative to littermate controls. This level is increased to an asymptomatic 37% if one ...

Severe inducible SMA mice have a neuromuscular phenotype

SMN2+/−; Smn2B-Neo/2B-Neo (hereafter referred to as severe inducible SMA) pups exhibited phenotypes similar to established severe models of SMA, including reduced survival (median survival, 7 d; p = 0.001), reduced weight (P2 or later; p ≤ 0.05), and diminished motor function (as quantified by tube test; P2 or later; p ≤ 0.01) (Fig. 1B–E) (Hsieh-Li et al., 2000; Monani et al., 2000; Le et al., 2005). Severe inducible SMA pups had near complete paralysis by P5 and never developed the ability to right when placed on their back. To assess overall health, we used electrocardiography (ECG) and found that severe inducible SMA mouse heart rates were significantly bradycardic from the earliest time point assayed (P3, SMA, 351 ± 95 bpm vs control, 462 ± 118 bpm; p = 0.04) and declined thereafter (Fig. 1F).

To confirm that the minimal level of excision (one allele per cell) would increase Smn to asymptomatic levels, we used breeding to replace one of the inducible alleles (Smn2B-Neo) with a Smn1tm1.1Cdid allele (referred to hereafter as Smn2B) that had already been induced by a E2A germline Cre. Western blot analysis confirmed SMN2+/−; Smn2B/2B-Neo pups had significantly increased Smn levels from 6 to 37% in P5 spinal cord (Fig. 1A). Importantly, this whole body rescue approach resulted in mice that survived over one year and were phenotypically indistinguishable from control littermates (data not shown). These experiments demonstrate that neomycin excision in even one of the two alleles is enough to correct the severe SMA-like phenotype documented in this model.

Presynaptic and postsynaptic defects in severe inducible SMA mice

To determine the extent of motor unit pathology in end-stage (P6) severe inducible SMA mice, we examined the fast-synapsing intercostal (IC) and the delayed synapsing triangularis sterni (TS) muscles. These muscles were chosen due to their role in maintaining proper respiratory function, one of the most critical deficits in human SMA patients.

The ICs of severe inducible SMA mice had a significant decrease in the number of fully innervated motor endplates (−36 ± 9%; p = 0.007) (Fig. 2A,B,E,F). This correlated with significant increases in both the number of partially occupied and denervated endplates. In contrast, TS NMJs were largely protected and did not significantly differ from controls (Fig. 2C–E,G). Hence, in this SMA model and time point, we consider the IC to be a vulnerable muscle and the TS to be a resistant muscle (McGovern et al., 2008; Ling et al., 2010).

Figure 2.
Severe inducible SMA mice have presynaptic and postsynaptic defects. A–D, Micrograph images depicting control (A, C) and mutant (B, D) IC and TS NMJs, respectively. E, Representative images of NMJs that have full innervation, have partial innervation, ...

Additionally, we assessed the postsynaptic architecture of αBTX-stained motor endplates, which are known to have delayed maturation in SMA mice (Murray et al., 2008; Kong et al., 2009). Relative to control littermates, severe inducible SMA pups had a 13 ± 4% (p = 0.05) increase in IC homogeneous motor endplates, and a 7 ± 0% (p = 0.04) decrease in the number of endplates containing secondary structure (Fig. 2H,I). Consistent with the innervation results, a similar pattern of protection was observed in the TS (Fig. 2J).

Finally, we quantified two classic presynaptic hallmarks of neurodegeneration: neurofilament accumulation and delayed/failed axonal pruning (Fig. 2H). We observed an 18 ± 5% (p = 0.03) increase in these presynaptic defects in SMA motor axons within the ICs, while SMA motor axons in the TS did not significantly differ from controls (Fig. 2I).

To place the pathology of our model in context with a commonly used model of SMA, we included the delta-7 mouse in our analysis (Le et al., 2005). Consistent with the milder phenotype at P6, the decrease in fully occupied NMJs (−15 ± 2%; p = 0.02) and the increase in partially occupied NMJs (+20 ± 4%; p = 0.02) within the ICs were all less dramatic in delta-7 mice relative to severe inducible SMA mice. Delta-7 and severe inducible SMA mice also demonstrated a parallel pattern of delayed motor endplate maturation and presynaptic defects (Fig. 2K,L) (Murray et al., 2008; Kong et al., 2009).

Hb9-Cre-driven recombination increases Smn expression in spinal MNs

The exact role of MNs in SMA remains an enigmatic mechanistic question. To address this point using severe inducible SMA mice, we used a Cre allele driven by the Hb9 promoter (Jax strain 6600) (Arber et al., 1999). In this widely used allele, Cre becomes active in all MNs and in a rare population of interneuron progenitors at embryonic day 9.5 (E9.5). It is of note that the prion promoter used in previous murine rescue experiments had a comparable temporal expression pattern, with expression being detected at E7.5 (Tremblay et al., 2007). Hb9-Cre is notably absent in a small percentage of lumbar MNs in the lateral motor column (LMC), but has robust expression in the cervical and thoracic spinal cord (Kramer et al., 2006). Importantly, it is not expressed in skeletal muscle, although minor amounts of excision were observed in kidney and stomach via PCR analysis (Fig. 3A). P5 mice doubly transgenic for Hb9-Cre and a ZGFP reporter allele were used to verify MN specificity, as only ChAT-positive MNs stained positive for GFP (with the rare exception of the Hb9 interneurons) (Fig. 3B) (Novak et al., 2000; Kramer et al., 2006).

Figure 3.
Specificity and efficiency of Hb9-Cre-driven recombination in vivo. A, A 3-primer PCR assay detects the presence or absence of the neomycin cassette in P5 MN-rescued SMA mice. Excision was observed in the spinal cord, with only minor amounts of promiscuous ...

We next bred the Hb9-Cre allele onto our severe inducible SMA background (hereafter referred to as MN-rescued SMA) and analyzed Smn levels in a variety of tissues via Western blot. In agreement with the expression pattern of Hb9-Cre, Smn levels increased slightly in the spinal cord (a dramatic increase would not be expected given the relatively small cellular contribution of MNs) (Fig. 3C). Importantly, there was no increase in Smn levels in the skeletal muscle, kidneys, or brain. To confirm Smn was increased in SMA motor neurons, we quantified nuclear gems, and found a significant increase in the average number of gems per MN in MN-rescued SMA mice (0.63 ± 0.11 gems; p ≤ 0.05) relative to severe inducible SMA mice (0.19 ± 0.02 gems) (Table 1). These results demonstrate that Hb9-Cre significantly increases Smn levels in MNs, while leaving peripheral tissues with SMA relevant Smn protein dosage.

Table 1.
Spinal motor neuron gem counts

Hb9-Cre significantly improves phenotype, but minimally improves survival

Having validated that Hb9-Cre was increasing Smn dosage exclusively in MNs, we assessed the phenotype of MN-rescued SMA mice. MN rescue dramatically improved the appearance and motor function of severe inducible SMA mice. While still runted, MN-rescued SMA pups had significantly improved righting reflex times (P7–P11; p ≤ 0.01) and were ambulatory throughout their entire life, a feature not seen in other severe SMA models (Fig. 4A–C). MN-rescued SMA mice also had significantly improved tube test scores (P8–P10; p ≤ 0.05) that improved steadily with age (Fig. 4D). Strangely, MN-rescued SMA mice exhibited a decreased level of consciousness or lethargy early in life that was not observed in severe inducible SMA mice or in control littermates, with or without Hb9-Cre. In these instances, MN-rescued SMA mice refused to attempt the righting reflex and tube tests, despite having the functional ability to successfully complete each test. The pups outgrew this passive behavior after P6; however, its presence resulted in poor motor function scores early in life (Fig. 4C,D).

Figure 4.
MN-rescued SMA mice have improved motor function, but minimally improved survival. A, Gross phenotype of severe inducible SMA mice is improved by Hb9-Cre. Pups are numbered using a white paint pen. B, Despite improved motor function, MN-rescued SMA mice ...

Despite the improved motor function, median survival of MN-rescued SMA mice increased by only 5 d (p = 0.001) (Fig. 4E). At the end stage, MN-rescued SMA mice were ambulatory and did not have significant paralysis, demonstrating only lateral instability of their hind limbs. This is likely attributed to a loss of MNs within the lumbar LMC, which control muscles responsible for stability and demonstrate weak Hb9-Cre expression (discussed further in next section).

MN rescue improves SMA motor unit pathology

To determine whether MN rescue corrected the presynaptic and postsynaptic motor unit pathology observed in severe inducible SMA pups, we examined NMJs in the ICs and TS of control and end-stage MN-rescued SMA mutants (the end stage was phenotypically defined as 2 consecutive days of weight loss). After blinded quantification, analysis revealed no significant differences in innervation status, endplate maturity, or presynaptic defects in the ICs of control and MN-rescued SMA mice (Fig. 5A–C) (data not shown). The TS also had no difference in innervation status and demonstrated only a significant decrease in junctions containing secondary structure (−34 ± 6%; p = 0.04) (Fig. 5D,E).

Figure 5.
Hb9-Cre rescues motor unit pathology in SMA mice. A–C, At end stage, MN-rescued SMA NMJs within the ICs were indistinguishable from controls in innervation status and endplate maturity (n = 6 per genotype, >50 NMJs per mouse). D, E, NMJs ...

To discount the possibility that MNs outside of those that innervate the TS and ICs were affected by disease, we quantified ChAT and Islet-1/2 double-positive MNs in the cervical, thoracic, and lumbar spinal cords of control, severe inducible, and MN-rescued SMA pups at end stage (Fig. 3F). In severe inducible SMA mice, a significant loss in average MNs per ventral horn of 4.4 ± 0.2, 4.1 ± 0.3, and 4.6 ± 1.3 was observed in cervical, thoracic, and lumbar spinal cords (p = 0.01, p = 0.04, and p = 0.05), respectively (Fig. 5G). In contrast, MN-rescued SMA spinal cords did not differ significantly from controls in the cervical and thoracic regions. A significant 5 ± 1 MN decrease was observed in L3–L5 spinal cord sections (p = 0.03) (Fig. 5G). This was not unanticipated, as the Hb9-Cre allele used here is known to have incomplete expression in the lumbar LMC (Kramer et al., 2006). A blinded postanalysis confirmed that the LMC in MN-rescued SMA mice presented with a 25 ± 9% reduction in MNs per ventral horn (p = 0.04), while the medial motor column (MMC) showed no significant decrease (Fig. 5H,I). These results support the conclusion that MN rescue is sufficient to prevent the neuromuscular pathology in our SMA model mice, since only MNs that appeared to be lost were those known to lack Hb9-Cre expression.

Hb9-Cre rescues loss of sensory-motor synapses

To determine the effect of MN rescue on glutamatergic excitatory synapses, which are known to be lost in delta-7 SMA mice, we quantified vGlut1-positive puncta juxtaposed to ChAT-positive MNs (Ling et al., 2010; Park et al., 2010; Mentis et al., 2011). End-stage (P5) severe inducible SMA mice had a significant reduction in the number of vGlut1-positive synapses per 100 μm perimeter when compared to control littermates (control, 3.67 ± 0.32 vs SMA, 2.74 ± 0.05; p = 0.04) (Fig. 5J,K). Conversely, MN-rescued SMA mice had significantly restored vGlut1 synapse numbers (3.92 ± 0.19; p ≤ 0.003) and were largely indistinguishable from controls (Fig. 5J,K). These results demonstrate that the loss of afferent synapses in SMA mice can be rescued by increasing Smn exclusively in MNs.

Hb9-Cre corrects SMA motor neuron hyperexcitability and excess synaptic activity

To confirm that SMA motor neurons rescued with Hb9-Cre were functionally normal, we performed whole-cell patch-clamp measurements on spinal MNs from P4–P5 control, SMA, and MN-rescued SMA mice. MNs from all three groups were indistinguishable in appearance, and stable recordings were readily achieved (Fig. 6A–C). There were no significant differences between the control, SMA, or MN-rescued SMA motor neurons in the resting membrane potential, whole-cell capacitance, input resistance, or action potential characteristics (all parameter values are provided in Table 2).

Figure 6.
Whole-cell patch clamp on medial MNs. A–C, Images representative of control, SMA, and MN-rescued SMA motor neurons. MNs were filled with Texas Red during recording. D, The current command shows the protocol of hyperpolarizing and depolarizing ...
Table 2.
Electrophysiological properties of motor neurons

Interestingly, the threshold voltage in SMA motor neurons was significantly lower (more hyperpolarized) relative to controls, and this phenotype was corrected in MN-rescued SMA motor neurons (Table 2). The amplitude of the persistent inward current (PIC) was significantly larger in SMA motor neurons and was restored to control levels by Hb9-Cre. Together, the changed PIC amplitude and threshold voltage parameters would suggest that increased excitability (hyperexcitability) is a property of SMA motor neurons that can be corrected by rescuing Smn levels exclusively within MNs.

Normally, it is not necessary to add blockers of synaptic activity to this preparation since there is minimal spontaneous synaptic activity in the quiescent preparation, though much of the circuitry remains intact. However, there was an unusually high frequency of postsynaptic potentials (PSPs) in SMA motor neurons, as shown in the voltage traces in Figure 6D–G. This was quantified as a significant increase in the number of potentials per second in severe inducible SMA mice (12.4 ± 5.1; p = 0.05) relative to control littermates (3.3 ± 0.3). Importantly, MN-rescued SMA motor neurons did not show increased PSPs relative to control littermates (2.5 ± 0.6) (Table 2). These results highlight the fact that alterations in motor circuitry are concomitant with alterations in the intrinsic properties of SMA motor neurons, since Hb9-Cre abolished the increased frequency of postsynaptic potentials.

MN-rescued SMA mice have autonomic defects

The degree of improvement observed in motor function, pathology, and electrophysiology makes it unlikely that NMJ dysfunction is the underlying cause of lethality in MN-rescued SMA pups. In recent years, a number of non-neuromuscular defects have been observed in SMA mice that could additively contribute to lethality in the absence of paralysis, one of which is cardiac defects (Bevan et al., 2010; Heier et al., 2010a; Shababi et al., 2010). Since we observed bradyarrhythmia in our severe inducible SMA mice and have previously documented similar findings in delta-7 SMA mice (Heier et al., 2010a), we assessed its presence as a contributing factor to lethality in MN-rescued SMA mutants. Unlike SMA mice without induction, MN-rescued SMA pups did not present with cardiac defects quantifiable by ECG early in life. However, by P9, mutants began to exhibit significant and progressive bradycardia (MN-rescued SMA, 503 ± 32 bpm vs control, 688 ± 9 bpm; p = 0.001) (Fig. 7A,B). Similar to what has been reported in delta-7 mice, end-stage MN-rescued SMA mice had signs of terminal heart block that manifested as skipped or dropped beats (Fig. 7B) (Heier et al., 2010a).

Figure 7.
MN-rescued SMA mice have deficits in autonomic control of the heart. A, B, The heart rate of MN-rescued SMA mice (n = 7) did not differ from controls (n = 14) early in life. However, at P9, MN-rescued SMA mice became significantly bradycardic (p ...

We further analyzed the components of ECG, such as the PR interval, QT interval, and QRS interval (Fig. 7C). Severe inducible SMA mice had significantly longer PR, QT, and QRS intervals at all time points examined (P3–P7; p < 0.05) (Fig. 7D–F). In contrast, MN-rescued SMA mice did not differ from controls early in life, but did exhibit significantly longer PR and QT intervals from P9 to P11 (p < 0.01 and p < 0.05, respectively) (Fig. 7D,E). MN-rescued SMA mice did not display any alterations in QRS interval (Fig. 7F). These results indicate that the ability of the myocardium to contract in response to ventricular depolarization was unaffected by disease (QRS), while the cardiac nervous system demonstrated delays in electrical conductance (PR and QT).

Previously, we demonstrated reduced sympathetic neuron staining and axon branches in the hearts of delta-7 SMA mice; however, it was unclear whether this was a primary deficit or a secondary complication of muscle weakness (Heier et al., 2010a). To assess the cardiac autonomic innervation pattern in MN-rescued SMA mice, who do not demonstrate significant paralysis, we performed tyrosine hydroxylase (TH) staining on control, SMA, and MN-rescued SMA mice. After standardizing the size of control and mutant hearts digitally using Photoshop, an average of 14 ± 0.5 major visible branches was quantified in control mice. In contrast, a significant reduction to 10 ± 1 and 11 ± 1 visible branches was observed in SMA and MN-rescued SMA mice (p = 0.02 and p = 0.008), respectively (Fig. 7G,H). Importantly, these defects in autonomic innervation exist in the absence of significant paralysis and/or motor unit pathology. This suggests that they are primary defects that likely combine with other non-neuromuscular defects and additively contribute to the poor health of SMA mice, both in the presence and absence of motor unit dysfunction.


Here we describe a novel mouse model of SMA with the ability to increase Smn dosage to asymptomatic levels after exposure to Cre-recombinase. Our model presents with severe SMA-like symptoms and pathology that are most similar to the severe model described by Monani et al. (2000) (Jax strain 5024). The experiments described in this manuscript demonstrate that MN rescue with Hb9-Cre can significantly improve motor function and motor unit pathology, which are commonly deficient in SMA mice. Furthermore, electrophysiology demonstrates that increasing Smn specifically within MNs is sufficient to correct hyperexcitability in SMA MNs, as well as abolish aberrant synaptic input to MNs.

Involvement of pathology outside the CNS

Despite a lack of significant paralysis, median survival is only extended 5 d in MN-rescued SMA mice. Our results, combined with those of Park et al. (2010), indicate that defects external to the MN exasperate the SMA phenotype by compromising the overall health of the mouse, but future experiments are required to definitively confirm this. One potential caveat to this interpretation is that inefficient Cre excision could be the root of lethality in our model and the cause of recovery in the Olig2-Cre SMA mice (Park et al., 2010). While unlikely, such a result would further emphasize the importance of MNs in the SMA phenotype, since a dramatic change in phenotype would be observed despite inefficient recombination. We attribute lethality in MN-rescued SMA mice, in part, to autonomic deficits in cardiac innervation and resulting heart failure. However, the severe phenotype in this model makes it probable that additional, non-neuromuscular factors also contribute to the observed lethality. Interestingly, there is mounting evidence to suggest that other cell types such as hepatocytes, osteoclasts, and myofibers may be affected in SMA mice, although it is unclear whether these defects are primary or secondary (Guettier-Sigrist et al., 2002; Araujo Ade et al., 2009; Shanmugarajan et al., 2009; Bevan et al., 2010; Heier et al., 2010a; Shababi et al., 2010; Wishart et al., 2010; Hua et al., 2011; Mutsaers et al., 2011). Despite the presence of non-neuromuscular phenotypes in severe SMA mice, it remains clear that long-term survival can be achieved with predominantly CNS-specific SMN rescue (Gavrilina et al., 2008; Foust et al., 2010; Passini et al., 2010, 2011; Hua et al., 2011; Osman et al., 2011).

MN pathology supports defects in central spinal circuitry

Several recent reports indicate that loss of the primary afferents that synapse onto MNs is an early hallmark and potentially significant contributor or mechanistic root of the SMA phenotype in mice (Ling et al., 2010; Park et al., 2010; Mentis et al., 2011). As has been noted in other SMA mouse models, the level of MN electrophysiological dysfunction quantified in our model is not sufficient to explain the significant reduction in motor function that exists (Zhang et al., 2010; Mentis et al., 2011). Given the high safety factor for neuromuscular transmission, the synaptic transmission defects that have been described in delta-7 SMA mice are also unlikely, on their own, to account for the observed phenotype (Kong et al., 2009; Ling et al., 2010; Ruiz et al., 2010). Hence, in our model the presence of hyperexcitable MNs, which experience an increased frequency of postsynaptic events and a loss of glutamatergic synapses, supports the conclusion that defects in spinal circuitry above the NMJ, such as sensory-motor synapses, play a significant role in driving the progression of a SMA-like disease in mice and potentially human SMA patients.

Here, we show an increased frequency of postsynaptic events in SMA MNs, whereas a previous study demonstrated decreased afferent input (Mentis et al., 2011). On the surface, these results appear to conflict; however, they are not mutually exclusive. Since synaptic formation and maintenance is altered between proprioceptive, vGlut1-expressing neurons and MNs, the formation and maintenance of synaptic contacts with other neurons, for example, local spinal interneurons that do not express vGlut1, could be altered as well. Therefore, deficits in afferent input are potentially part of the same altered circuitry that is responsible for the increased spontaneous synaptic activity.

In addition to Hb9-positive MNs, another group of neurons could be involved in the rescued phenotype: the Hb9 interneurons. This small population of glutamatergic interneurons (~40 per segment) is present in limited thoracic and lumbar spinal cord segments, T13–L3 (Hinckley et al., 2005; Wilson et al., 2005; Kwan et al., 2009). They receive monosynaptic input from sensory afferents (Hinckley et al., 2010) and have sparse synaptic contacts with MNs (Hinckley et al., 2005; Wilson et al., 2005). Since Hb9 interneurons are also rescued, it could be argued that loss of Smn protein renders them hyperexcitable, and their subsequent rescue explains the absence of aberrant synaptic activity. However, this is highly improbable, since contacts between Hb9 interneurons and MNs are rare (Wilson et al., 2005), and based on their low levels of activity during activation of the locomotor network, the possibility that these interneurons drive another population of premotor interneurons in quiescent cord appears somewhat remote (Kwan et al., 2009).

Pathology of MNs

Some of the findings here are not identical to those of previous studies. In this SMA model, we did not observe changes in input resistance or action potential height, as was reported in Mentis et al. (2011). This may be due to the different SMA models or the preparations used (whole isolated spinal cord vs spinal cord slice). However, our observations are similar to previous studies in that the threshold voltage of SMA MNs is more hyperpolarized, which would allow them to fire with less depolarizing input (Zhang et al., 2010; Mentis et al., 2011). Increased excitability, including an increased persistent inward current, has been observed in other conditions of spinal MN dysfunction, such as spinal cord injury and MN disease (Li and Bennett, 2003; Kuo et al., 2005; Harvey et al., 2006; Meehan et al., 2010; Quinlan et al., 2011). This might indicate that MN excitability is a common thread in SMA and, more broadly, in MN pathology.

Defects in sensory-motor synapses are specific to MNs

Aberrant synaptic activity in SMA can be explained by altered synapse development and maintenance. Since synaptic integrity requires faithful and reciprocal presynaptic and postsynaptic signaling, the loss of sensory-MN interaction could be due to a failure of primary afferents to deliver appropriate neurotransmitters across the synapse. Alternatively, the inability of the postsynaptic MN to maintain normal levels of excitability could result in the loss of primary afferent synapses, while other synaptic contacts are upregulated. Results from this study would argue that the latter is the mechanism of afferent synapse loss in SMA, since our MN-rescued SMA mice, who express only asymptomatic levels of Smn in MNs, do not show a loss in vGlut1 bouton number or evidence of altered synaptic inputs. This finding is in agreement with the previous observation that sensory-motor synapses are lost in mice that have normal Smn dosage in all cells except MNs and oligodendrocytes (Park et al., 2010).

The existence of non-neuromuscular contributions to lethality makes it challenging to determine whether, with prolonged survival, aberrant synaptic activity in Hb9-Cre-rescued SMA motor neurons would develop; however, dissecting this will require milder inducible models of SMA than the one described here. Together, these findings suggest that the role of the postsynaptic cell should not be underestimated in maintenance of afferent synapses.


Collectively, our results and those of others indicate that deficits in the central circuit play a significant role in SMA disease progression and paralysis in severe SMA mice and potentially human SMA patients (Ling et al., 2010; Park et al., 2010; Mentis et al., 2011). Moreover, our results support the idea that loss of sensory-motor synapses is a consequence, and not a cause, of MN dysfunction. Finally, this work demonstrates that neuromuscular dysfunction in SMA mice is mechanistically due to deficits within MNs. These defects are enhanced by the presence of additional primary or secondary defects, all of which act additively to comprise the general health of the mouse. As such, this work does not rule out the potentially significant benefits of restoring Smn within the other components of the motor unit, such as skeletal muscle and/or Schwann cells, which may play important roles in defining disease severity. Future work determining how many rescued MNs are required to affect a phenotypic benefit will have important implications in developing effective therapies to treat SMA patients.


This work was supported by NIH Training Grant T32 AG000260, Drug Discovery Training in Age-Related Disorders (R.G.), Families of Spinal Muscular Atrophy Grant DiD0809 (C.J.D.), and NIH NINDS Grants 1ROIN5060926 (C.J.D.), 3RO1NS060926-02S3 (C.J.D.), NS034382 (C.J.H.), and NS071951 (C.J.H., K.A.Q.). K.A.Q. made use of equipment supported by NS054850. We acknowledge Herminio Cardona's and Michael Jorgensen's roles in overall colony maintenance, Carina Emery for experimental assistance, as well as the labs of Dr. Greg Cox and Dr. Robert Burgess for technical training rendered.

The authors declare no competing financial interests.


Araujo Ade et al., 2009. Araujo Ade Q, Araujo M, Swoboda KJ. Vascular perfusion abnormalities in infants with spinal muscular atrophy. J Pediatr. 2009;155:292–294. [PMC free article] [PubMed]
Arber et al., 1999. Arber S, Han B, Mendelsohn M, Smith M, Jessell TM, Sockanathan S. Requirement for the homeobox gene Hb9 in the consolidation of motor neuron identity. Neuron. 1999;23:659–674. [PubMed]
Bevan et al., 2010. Bevan AK, Hutchinson KR, Foust KD, Braun L, McGovern VL, Schmelzer L, Ward JG, Petruska JC, Lucchesi PA, Burghes AH, Kaspar BK. Early heart failure in the SMNDelta7 model of spinal muscular atrophy and correction by postnatal scAAV9-SMN delivery. Hum Mol Genet. 2010;19:3895–3905. [PMC free article] [PubMed]
Boon et al., 2009. Boon KL, Xiao S, McWhorter ML, Donn T, Wolf-Saxon E, Bohnsack MT, Moens CB, Beattie CE. Zebrafish survival motor neuron mutants exhibit presynaptic neuromuscular junction defects. Hum Mol Genet. 2009;18:3615–3625. [PMC free article] [PubMed]
Briese et al., 2009. Briese M, Esmaeili B, Fraboulet S, Burt EC, Christodoulou S, Towers PR, Davies KE, Sattelle DB. Deletion of smn-1, the Caenorhabditis elegans ortholog of the spinal muscular atrophy gene, results in locomotor dysfunction and reduced lifespan. Hum Mol Genet. 2009;18:97–104. [PMC free article] [PubMed]
Chang et al., 2008. Chang HC, Dimlich DN, Yokokura T, Mukherjee A, Kankel MW, Sen A, Sridhar V, Fulga TA, Hart AC, Van Vactor D, Artavanis-Tsakonas S. Modeling spinal muscular atrophy in Drosophila. PLoS One. 2008;3:e3209. [PMC free article] [PubMed]
Coovert et al., 1997. Coovert DD, Le TT, McAndrew PE, Strasswimmer J, Crawford TO, Mendell JR, Coulson SE, Androphy EJ, Prior TW, Burghes AH. The survival motor neuron protein in spinal muscular atrophy. Hum Mol Genet. 1997;6:1205–1214. [PubMed]
Crawford and Pardo, 1996. Crawford TO, Pardo CA. The neurobiology of childhood spinal muscular atrophy. Neurobiol Dis. 1996;3:97–110. [PubMed]
DiDonato et al., 2003. DiDonato CJ, Parks RJ, Kothary R. Development of a gene therapy strategy for the restoration of survival motor neuron protein expression: implications for spinal muscular atrophy therapy. Hum Gene Ther. 2003;14:179–188. [PubMed]
Foust et al., 2010. Foust KD, Wang X, McGovern VL, Braun L, Bevan AK, Haidet AM, Le TT, Morales PR, Rich MM, Burghes AH, Kaspar BK. Rescue of the spinal muscular atrophy phenotype in a mouse model by early postnatal delivery of SMN. Nat Biotechnol. 2010;28:271–274. [PMC free article] [PubMed]
Gavrilina et al., 2008. Gavrilina TO, McGovern VL, Workman E, Crawford TO, Gogliotti RG, DiDonato CJ, Monani UR, Morris GE, Burghes AH. Neuronal SMN expression corrects spinal muscular atrophy in severe SMA mice while muscle-specific SMN expression has no phenotypic effect. Hum Mol Genet. 2008;17:1063–1075. [PMC free article] [PubMed]
Guettier-Sigrist et al., 2002. Guettier-Sigrist S, Hugel B, Coupin G, Freyssinet JM, Poindron P, Warter JM. Possible pathogenic role of muscle cell dysfunction in motor neuron death in spinal muscular atrophy. Muscle Nerve. 2002;25:700–708. [PubMed]
Hammond et al., 2010. Hammond SM, Gogliotti RG, Rao V, Beauvais A, Kothary R, DiDonato CJ. Mouse survival motor neuron alleles that mimic SMN2 splicing and are inducible rescue embryonic lethality early in development but not late. PLoS One. 2010;5:e15887. [PMC free article] [PubMed]
Harvey et al., 2006. Harvey PJ, Li Y, Li X, Bennett DJ. Persistent sodium currents and repetitive firing in motoneurons of the sacrocaudal spinal cord of adult rats. J Neurophysiol. 2006;96:1141–1157. [PubMed]
Heier et al., 2010a. Heier CR, Satta R, Lutz C, DiDonato CJ. Arrhythmia and cardiac defects are a feature of spinal muscular atrophy model mice. Hum Mol Genet. 2010a;19:3906–3918. [PMC free article] [PubMed]
Heier et al., 2010b. Heier CR, Hampton TG, Wang D, Didonato CJ. Development of electrocardiogram intervals during growth of FVB/N neonate mice. BMC Physiol. 2010b;10:16. [PMC free article] [PubMed]
Hinckley et al., 2005. Hinckley CA, Hartley R, Wu L, Todd A, Ziskind-Conhaim L. Locomotor-like rhythms in a genetically distinct cluster of interneurons in the mammalian spinal cord. J Neurophysiol. 2005;93:1439–1449. [PubMed]
Hinckley et al., 2010. Hinckley CA, Wiesner EP, Mentis GZ, Titus DJ, Ziskind-Conhaim L. Sensory modulation of locomotor-like membrane oscillations in Hb9-expressing interneurons. J Neurophysiol. 2010;103:3407–3423. [PubMed]
Hsieh-Li et al., 2000. Hsieh-Li HM, Chang JG, Jong YJ, Wu MH, Wang NM, Tsai CH, Li H. A mouse model for spinal muscular atrophy. Nat Genet. 2000;24:66–70. [PubMed]
Hua et al., 2011. Hua Y, Sahashi K, Rigo F, Hung G, Horev G, Bennett CF, Krainer AR. Peripheral SMN restoration is essential for long-term rescue of a severe spinal muscular atrophy mouse model. Nature. 2011;478:123–126. [PMC free article] [PubMed]
Kong et al., 2009. Kong L, Wang X, Choe DW, Polley M, Burnett BG, Bosch-Marce M, Griffin JW, Rich MM, Sumner CJ. Impaired synaptic vesicle release and immaturity of neuromuscular junctions in spinal muscular atrophy mice. J Neurosci. 2009;29:842–851. [PMC free article] [PubMed]
Kramer et al., 2006. Kramer ER, Knott L, Su F, Dessaud E, Krull CE, Helmbacher F, Klein R. Cooperation between GDNF/Ret and ephrinA/EphA4 signals for motor-axon pathway selection in the limb. Neuron. 2006;50:35–47. [PubMed]
Kuo et al., 2005. Kuo JJ, Siddique T, Fu R, Heckman CJ. Increased persistent Na+ current and its effect on excitability in motoneurones cultured from mutant SOD1 mice. J Physiol. 2005;563:843–854. [PubMed]
Kwan et al., 2009. Kwan AC, Dietz SB, Webb WW, Harris-Warrick RM. Activity of Hb9 interneurons during fictive locomotion in mouse spinal cord. J Neurosci. 2009;29:11601–11613. [PMC free article] [PubMed]
Le et al., 2005. Le TT, Pham LT, Butchbach ME, Zhang HL, Monani UR, Coovert DD, Gavrilina TO, Xing L, Bassell GJ, Burghes AH. SMNDelta7, the major product of the centromeric survival motor neuron (SMN2) gene, extends survival in mice with spinal muscular atrophy and associates with full-length SMN. Hum Mol Genet. 2005;14:845–857. [PubMed]
Le et al., 2011. Le TT, McGovern VL, Alwine IE, Wang X, Massoni-Laporte A, Rich MM, Burghes AH. Temporal requirement for high SMN expression in SMA mice. Hum Mol Genet. 2011;20:3578–3591. [PMC free article] [PubMed]
Lefebvre et al., 1995. Lefebvre S, Bürglen L, Reboullet S, Clermont O, Burlet P, Viollet L, Benichou B, Cruaud C, Millasseau P, Zeviani M, et al. Identification and characterization of a spinal muscular atrophy-determining gene. Cell. 1995;80:155–165. [PubMed]
Lefebvre et al., 1997. Lefebvre S, Burlet P, Liu Q, Bertrandy S, Clermont O, Munnich A, Dreyfuss G, Melki J. Correlation between severity and SMN protein level in spinal muscular atrophy. Nat Genet. 1997;16:265–269. [PubMed]
Li and Bennett, 2003. Li Y, Bennett DJ. Persistent sodium and calcium currents cause plateau potentials in motoneurons of chronic spinal rats. J Neurophysiol. 2003;90:857–869. [PubMed]
Ling et al., 2010. Ling KK, Lin MY, Zingg B, Feng Z, Ko CP. Synaptic defects in the spinal and neuromuscular circuitry in a mouse model of spinal muscular atrophy. PLoS One. 2010;5:e15457. [PMC free article] [PubMed]
McGovern et al., 2008. McGovern VL, Gavrilina TO, Beattie CE, Burghes AH. Embryonic motor axon development in the severe SMA mouse. Hum Mol Genet. 2008;17:2900–2909. [PMC free article] [PubMed]
Meehan et al., 2010. Meehan CF, Moldovan M, Marklund SL, Graffmo KS, Nielsen JB, Hultborn H. Intrinsic properties of lumbar motor neurones in the adult G127insTGGG superoxide dismutase-1 mutant mouse in vivo: evidence for increased persistent inward currents. Acta Physiol. 2010;200:361–376. [PubMed]
Mentis et al., 2011. Mentis GZ, Blivis D, Liu W, Drobac E, Crowder ME, Kong L, Alvarez FJ, Sumner CJ, O'Donovan MJ. Early functional impairment of sensory-motor connectivity in a mouse model of spinal muscular atrophy. Neuron. 2011;69:453–467. [PMC free article] [PubMed]
Monani et al., 2000. Monani UR, Sendtner M, Coovert DD, Parsons DW, Andreassi C, Le TT, Jablonka S, Schrank B, Rossol W, Prior TW, Morris GE, Burghes AH. The human centromeric survival motor neuron gene (SMN2) rescues embryonic lethality in Smn(−/−) mice and results in a mouse with spinal muscular atrophy. Hum Mol Genet. 2000;9:333–339. [PubMed]
Murray et al., 2008. Murray LM, Comley LH, Thomson D, Parkinson N, Talbot K, Gillingwater TH. Selective vulnerability of motor neurons and dissociation of pre- and post-synaptic pathology at the neuromuscular junction in mouse models of spinal muscular atrophy. Hum Mol Genet. 2008;17:949–962. [PubMed]
Mutsaers et al., 2011. Mutsaers CA, Wishart TM, Lamont DJ, Riessland M, Schreml J, Comley LH, Murray LM, Parson SH, Lochmüller H, Wirth B, Talbot K, Gillingwater TH. Reversible molecular pathology of skeletal muscle in spinal muscular atrophy. Hum Mol Genet. 2011;20:4334–4344. [PubMed]
Novak et al., 2000. Novak A, Guo C, Yang W, Nagy A, Lobe CG. Z/EG, a double reporter mouse line that expresses enhanced green fluorescent protein upon Cre-mediated excision. Genesis. 2000;28:147–155. [PubMed]
Osman et al., 2011. Osman EY, Yen PF, Lorson CL. Bifunctional RNAs targeting the intronic splicing silencer N1 increase SMN levels and reduce disease severity in an animal model of spinal muscular atrophy. Mol Ther. 2011;20:119–126. [PubMed]
Park et al., 2010. Park GH, Maeno-Hikichi Y, Awano T, Landmesser LT, Monani UR. Reduced survival of motor neuron (SMN) protein in motor neuronal progenitors functions cell autonomously to cause spinal muscular atrophy in model mice expressing the human centromeric (SMN2) gene. J Neurosci. 2010;30:12005–12019. [PMC free article] [PubMed]
Passini et al., 2010. Passini MA, Bu J, Roskelley EM, Richards AM, Sardi SP, O'Riordan CR, Klinger KW, Shihabuddin LS, Cheng SH. CNS-targeted gene therapy improves survival and motor function in a mouse model of spinal muscular atrophy. J Clin Invest. 2010;120:1253–1264. [PMC free article] [PubMed]
Passini et al., 2011. Passini MA, Bu J, Richards AM, Kinnecom C, Sardi SP, Stanek LM, Hua Y, Rigo F, Matson J, Hung G, Kaye EM, Shihabuddin LS, Krainer AR, Bennett CF, Cheng SH. Antisense oligonucleotides delivered to the mouse CNS ameliorate symptoms of severe spinal muscular atrophy. Sci Transl Med. 2011;3:72ra18. [PMC free article] [PubMed]
Pellizzoni et al., 1998. Pellizzoni L, Kataoka N, Charroux B, Dreyfuss G. A novel function for SMN, the spinal muscular atrophy disease gene product, in pre-mRNA splicing. Cell. 1998;95:615–624. [PubMed]
Quinlan et al., 2011. Quinlan KA, Schuster JE, Fu R, Siddique T, Heckman CJ. Altered postnatal maturation of electrical properties in spinal motoneurons in a mouse model of amyotrophic lateral sclerosis. J Physiol. 2011;589:2245–2260. [PubMed]
Ruiz et al., 2010. Ruiz R, Casañas JJ, Torres-Benito L, Cano R, Tabares L. Altered intracellular Ca2+ homeostasis in nerve terminals of severe spinal muscular atrophy mice. J Neurosci. 2010;30:849–857. [PubMed]
Schrank et al., 1997. Schrank B, Götz R, Gunnersen JM, Ure JM, Toyka KV, Smith AG, Sendtner M. Inactivation of the survival motor neuron gene, a candidate gene for human spinal muscular atrophy, leads to massive cell death in early mouse embryos. Proc Natl Acad Sci U S A. 1997;94:9920–9925. [PubMed]
Shababi et al., 2010. Shababi M, Habibi J, Yang HT, Vale SM, Sewell WA, Lorson CL. Cardiac defects contribute to the pathology of spinal muscular atrophy models. Hum Mol Genet. 2010;19:4059–4071. [PubMed]
Shanmugarajan et al., 2009. Shanmugarajan S, Tsuruga E, Swoboda KJ, Maria BL, Ries WL, Reddy SV. Bone loss in survival motor neuron (Smn(−/−) SMN2) genetic mouse model of spinal muscular atrophy. J Pathol. 2009;219:52–60. [PMC free article] [PubMed]
Tremblay et al., 2007. Tremblay P, Bouzamondo-Bernstein E, Heinrich C, Prusiner SB, DeArmond SJ. Developmental expression of PrP in the post-implantation embryo. Brain Res. 2007;1139:60–67. [PMC free article] [PubMed]
Wilson et al., 2005. Wilson JM, Hartley R, Maxwell DJ, Todd AJ, Lieberam I, Kaltschmidt JA, Yoshida Y, Jessell TM, Brownstone RM. Conditional rhythmicity of ventral spinal interneurons defined by expression of the Hb9 homeodomain protein. J Neurosci. 2005;25:5710–5719. [PubMed]
Wishart et al., 2010. Wishart TM, Huang JP, Murray LM, Lamont DJ, Mutsaers CA, Ross J, Geldsetzer P, Ansorge O, Talbot K, Parson SH, Gillingwater TH. SMN deficiency disrupts brain development in a mouse model of severe spinal muscular atrophy. Hum Mol Genet. 2010;19:4216–4228. [PMC free article] [PubMed]
Zhang et al., 2010. Zhang H, Robinson N, Wu C, Wang W, Harrington MA. Electrophysiological properties of motor neurons in a mouse model of severe spinal muscular atrophy: in vitro versus in vivo development. PLoS One. 2010;5:e11696. [PMC free article] [PubMed]

Articles from The Journal of Neuroscience are provided here courtesy of Society for Neuroscience