The neurons that restore walking after paralysis
Study design and participants
All experiments were carried out as part of the ongoing clinical feasibility study STIMO, which investigates the effects of spatiotemporal EES combined with weight-supported overground locomotor training on the recovery of motor function after SCI (clinicaltrials.gov, NCT02936453). The context, primary and secondary endpoints, and timeline of the study are described in Supplementary Note 1. This study was approved by the Swiss ethical authorities (Swissethics protocol number 04/2014 ProjectID: PB_2016-00886, Swissmedic protocol 2016-MD-0002) and was conducted in accordance with the Declaration of Helsinki. All participants provided written informed consent prior to their participation. All surgical and experimental procedures were performed at the Lausanne University Hospital (CHUV) and have been previously described in detail1. The study involved assessments before surgery, the surgical implantation of the neurostimulation system, a one-month period during which EES protocols were configured, and a five-month rehabilitation period with physiotherapists taking place four to five times per week for one to three hours. The rehabilitation programme was personalized based on the participants’ improvements. At the end of the rehabilitation period, the participants were given the opportunity to be enroled in a study extension phase during which they could continue using the neurostimulation system at home. They are currently followed-up on a regular basis by the study team for up to six years. To date, a total of nine individuals completed the main part of the study. Their neurological status was evaluated according to the International Standards for Neurological Classification of Spinal Cord Injury (ISNCSCI), and is reported in Supplementary Table 1. The outcomes from these nine individuals are reported in this report.
In humans, EES was delivered using a paddle lead that was surgically implanted over the epidural surface of the lumbar spinal cord. The first 6 participants were implanted with the Specify 5-6-5 paddle lead, which was originally designed to target the dorsal column in order to alleviate pain (Specify 5-6-5, Medtronic). The last three participants were implanted with a new paddle lead that was specifically developed to target the dorsal roots involved in the control of trunk and leg movements18 (ONWARD Medical). The paddle leads were connected to an implantable pulse generator (IPG) (Medtronic Activa RC, Medtronic) commonly used for deep-brain stimulation therapies. We upgraded this IPG with a wireless communication bridge that enabled real-time control over the parameters of EES protocols.
Since the participants were equipped with implanted medical devices that were not approved for MRI, we measured the spinal cord glucose consumption as a surrogate of neuronal activity during walking using non-invasive FDG-PET–computed tomography (PET/CT) imaging after walking. This technique was previously used to study the effect of spinal cord stimulation at the cervical level52. PET scans were acquired four weeks after the surgical implantation of the devices and after EESREHAB with EESON, using 150 MBq of FDG. Participants were asked to walk for the first 15 min of the FDG uptake. If participants were not able to walk prior to rehabilitation, they were asked to hold onto a Taurus and attempt to walk while their legs were moved by physiotherapists. Spinal cord FDG uptake was then measured at 45 min after radiotracer injection with 3 min per bed position, and assessed in SUVbw, from T10 to L2 vertebral body levels using CT images for anatomic localization. The SUVbw index represents the FDG uptake by the neuron cell bodies and dendritic processes forming the grey matter, corrected for injected radiotracer activity, radioactive decay and body weight53. Glucose consumption was compared before and after EESREHAB using a mixed effect linear model. PET images were also coregistered in a preoperative 3D MRI scan of the spinal cord for visualization purposes.
Neurological status was assessed based on the ISNCSCI54, a comprehensive clinician-administered neurological examination of residual sensory and motor function quantifying SCI severity.
Participants followed a neurorehabilitation programme four to five times per week for five months. The programme was personalized to participants’ performance, but generally comprised a mixture of walking on a treadmill and overground with multiple assistive devices, sit-to-stand, standing, leg and trunk muscle exercises, swimming and cycling. Activity-specific stimulation programmes were delivered to enable the practice of these activities. The minimum amount of body weight support required to walk overground was recorded during monthly gait assessments.
Six-minute walk test
Endurance was assessed by the distance covered overground within six minutes with a standard four-wheel walker but without any external assistance55,56. This test was performed before and after EESREHAB with EESON and EESOFF.
Ten-metre walk test
Walking speed was assessed by a timed ten-metre walk test without any external assistance56. Only two participants were evaluated with 5% body weight support for safety (ST006, MB007). Participants were instructed to walk with the preferred assistive device as fast as they could. This test was performed before and after EESREHAB with EESON and EESOFF.
Recordings of muscle activity
Participants were lying relaxed in supine position on an examination table. Electromyographic (EMG) activity was recorded bilaterally from the iliopsoas (Il), rectus femoris (RF), vastus lateralis (VLat), semitendinosus (ST), tibialis anterior (TA), medial gastrocnemius (MG) and soleus (Sol) muscles with wireless bipolar surface electrodes (Myon 320, Myon or Delsys Trigno). Each electrode was placed centrally over the muscle with a longitudinal alignment and an inter-electrode distance of 3 cm. Abrasive paste (Nuprep, 4Weaver and Company) was used for skin preparation to reduce electrode-skin resistance and improve EMG signal quality. Stimulation artefacts required for responses alignment were picked up by an additional pair of surface-EMG electrodes placed over the spine at the thoracolumbar junction or from the iliopsoas sensors ipsilateral to the IPG. Muscular recordings were acquired with Delsys Trigno Plugin v2.0.2 integrated in Nexus v1.8.5. Continuous EMG signals were sampled at 5 kHz (Myon) or 2 kHz (Delsys) and saved to a desktop computer. EMG signals were bandpass filtered between 20 and 450 Hz. Recordings were performed with graded stimulation amplitudes. Each contact of the implanted electrode array was stimulated in monopolar configuration as the cathode, with the case of the implantable pulse generator set as the anode. First, low-amplitude stimulation was applied to identify the lowest response threshold across all recorded muscles (motor threshold (MT)). Then, EES amplitude was increased manually to identify the amplitudes at which the responses reached a plateau, limited to levels that did not cause discomfort to the participant. Finally, single-pulse EES at amplitudes ranging from response threshold to saturation was performed automatically, with four repetitions at each EES amplitude. Recorded EMG responses were segmented in windows from 6–50 ms and from 50–100 ms for short and long-latency components of muscle responses. The amplitudes of each component were quantified as peak-to-peak. Ten long-latency stimulation responses in the range of 1.1–1.3 × MT were quantified.
Adult male or female C57BL/6 mice (15–35 g body weight, 12–30 weeks of age) or transgenic mice were used for all experiments. Vglut2cre (Jackson Laboratory 016963), Ai65(RCFL-tdT) (Jackson Laboratory 021875), Parvalbumin (PV)cre (Jackson Laboratory 017320), AdvillinFlpO (a gift from V. Abraira) and Vsx2cre (MMMRRC 36672, also called Chx10cre) transgenic mouse strains were bred and maintained on a mixed genetic background (C57BL/6). Housing, surgery, behavioural experiments and euthanasia were all performed in compliance with the Swiss Veterinary Law guidelines. Mice were maintained in house under standard housing conditions (12-h light/dark cycle) with 24 h access to water and standard chow diet at temperature at 21 ± 1 °C and relative humidity at 55 ± 5%. All procedures and surgeries were approved by the Veterinary Office of the Canton of Geneva. Manual bladder voiding and all other animal care was performed twice daily for the first three weeks after injury and once daily for the remaining period of experiment. All procedures and surgeries were approved by the Veterinary Office of the Canton of Geneva (Switzerland; license GE/25/17).
Viruses and virus production
Viruses used in this study were either acquired commercially or produced locally. The following AAV plasmids were used and detailed sequence information is available as detailed or upon request: AAVDj-hSyn-flex-mGFP-2A-synaptophysin-mRuby57 (Stanford Vector Core Facility, reference AAV DJ GVVC-AAV-100), AAV5-CAG-DIO-COMET-tdTomato and AAV5CAG-COMET-GFP (a gift from M. Tuszynski), AAV5-Syn-flex-ChrimsonR-tdT (Addgene 62723), AAV5-CAG-flex-Jaws-KGC-GFP-ER2 (Addgene 84445), AAV5-hSyn-DIO-hm4D (Gi)-mCherry (Addgene 44362), AAV5-hSyn-DIO-hm3D (Gq)-mCherry (Addgene 44361), AAV5-CAG-flex-tdTomato (a gift from S. Arber), AAV5CAG-flex-human diphtheria toxin receptor (DTR) (a gift from S. Arber), AAV5-DIO-TC66T-2A-eGFP-2A-oG (GT3) (Salk Institute) and AAV5-hSyn-DIO-TVAP2A-EGFP-2A-oG (a gift from T. Karayannis). All floxed AAV vectors used in the present study showed transgene expression only upon Cre-mediated recombination. Trans-synaptic tracings were performed with EnvA-G-deleted rabies–mCherry (GT3) (Salk Institute 32646) or the cre-dependent PRV Ba2017 (expressing GFP; 4.9 × 109 pfu per ml; Princeton University). Injection volumes, coordinates and experimental purpose are described below.
General surgical procedures have been described previously in detail28. Surgeries were performed under aseptic conditions and under 1–2% isoflurane in 0.5–1 l min−1 flow of oxygen as general anaesthesia. After surgeries, mice were allowed to wake up in an incubator. Analgesia—buprenorphine (Essex Chemie, 0.01–0.05 mg kg−1 subcutaneous injection) or rimadyl (5 mg kg−1 subcutaneous injection)—was given twice daily for 2–3 days after surgery.
Spinal cord contusion and lateral hemisections were performed as previously described28. A laminectomy was made at the mid-thoracic level (T8 and T9 vertebra). To perform a contusion injury, we used a force-controlled spinal cord impactor58 (IH-0400 Impactor, Precision Systems and Instrumentation), as previously described28. The applied force was set to 95 kDyn. Hemisections were performed at the mid-thoracic level after a laminectomy (T8 vertebra) using a microscalpel.
For lumbar cord injections for viral vector tracings, a laminectomy of T13 was performed and 4 injections were made on either side. For lumbar cord injections, which are followed by EES or spinal micro-array implantations, the interlaminar spaces between T12/T13, T13/L1 and L1/L2 were dissected. Injections were performed using a pulled glass pipette driven with the Nanoliter pump (Nanoliter 2010 injector, World Precision Instruments) fixed to a stereotaxic frame. Two injections were made on either side of the spinal cord per interlaminar space. Fifty nanolitres at a rate of 100 nl s−1 were injected at 0.6 mm and at 0.3 mm below the dorsal surface of the spinal cord.
An incision was made across the skull. To target corticospinal neurons in layer V motor cortex, bregma was identified and a craniotomy 1 mm–2 mm medial and −0.5 mm to 2 mm rostro-caudally was performed with a hand-held drill28. One-hundred nanolitre injections at 3 nl s−1 were made bilaterally at medial–lateral 1.2 mm and 1.7 mm, rostro-caudally at 0 mm, −0.5 mm, −1 mm and −1.5 mm, dorso-ventrally at a depth of 0.5 mm from the brain surface. To target descending neurons in the reticulospinal formation, bregma was identified and a craniotomy 5 mm-6 mm dorsal and 0 mm–2 mm lateral to Bregma was performed28. One-hundred nanolitre injections at 3 nl s−1 were made bilaterally at medial–lateral 0.3 mm, rostro-caudally at −5.8 mm and −6.2 mm, dorso-ventrally at a depth of 5.6 mm from the brain surface.
EES implantations and stimulation protocols
All the procedures have been detailed previously3,4,5,28,59,60. To position electrodes to deliver EES in mice, laminotomies (removal of only the connective tissue in between the bones, but not bones) were performed at T12/T13 and L1/L2 to expose the spinal cord. Tefloncoated stainless steel wires connected to a percutaneous connector (Omnetics Connector Corporation) were inserted on either side and passed between the spinal cord and the vertebral bones to the other opening. A small part of insulation was removed and the exposed stimulation sites were positioned over L2 and S1. A common ground was inserted subcutaneously. The percutaneous connector was cemented to the skull. Stimulation was therefore delivered to both sites simultaneously. Conventional stimulation protocols consisted of continuous EES delivered at 40 Hz with 0.2 ms pulses at 50–300 µA. High-frequency burst stimulation protocols consisted of 10-ms-long bursts of 0.2-ms-long pulses, 50–300 µA at 600 Hz with a modulating frequency of 30 Hz. This high-frequency burst stimulation protocol was subsequently used for all acute and chronic experiments.
Photostimulation of the motor cortex
All the procedures have been detailed previously25,26,27,28. In the same surgical procedure as brain injections into the motor cortex, optic fibres (200 µm core diameter, 9.22 NA, Thorlabs) passed through 1.25 mm ceramic ferrules (CFLC126-10, Thorlabs) were implanted bilaterally at 0.5 mm lateral and 0.5 mm caudal to Bregma at a depth of 0.5 mm. Three screws (AMS120/5B25, Antrin Miniature Specialties) were inserted into the skull, surrounding the ferrules connector. Fresh dental cement was then poured around the screws and ferrules, and left until cured. Light was transmitted through a ferrule-to ferrule connection. A blue laser (laserglow, 473 nm Blue DPSS Laser System) was used to photostimulate the cortex every 5 s over 3 s and consisted of 10 ms long pulses28 at 40 Hz.
Chronic implantation of electrodes to record muscle activity
All the procedures have been detailed previously3,4,5,28,60. An incision over the muscle of interest (tibialis anterior, gastrocnemius) was made and if needed the muscle was exposed by blunt dissection of overlying tissue. Bipolar intramuscular electrodes were inserted into the muscle parallel to the muscle fibre orientation. To confirm optimal placing, the wires were electrically stimulated resulting in a muscle. Electrodes were fixed in place by suturing either side of the electrode that exited the muscle 45. A grounding wire was implanted subcutaneously. Wires were connected to a percutaneous connector (Omnetics Connector Corporation) cemented to the skull. Electromyographic signals (2 kHz) were amplified (1k), filtered (100–1k bandwidth, A-M Systems Differential AC Amplifier Model 1700) and digitalized either with the Vicon System or with the Powerlab system (AdInstruments).
EESREHAB in mice
One week after contusion injury, mice were trained daily for four weeks. Five minutes before training, the mice received a small bolus of quipazine (5-HT2A/C, 0.2–0.3 mg kg−1) and intraperitoneal injections of 8-OH-DPAT (5HT1A/7, 0.05-0.2 mg kg−1) to reactivate the lumbar spinal neurons and to enable sustained locomotion during neurorehabilitation4. The dose was progressively reduced during recovery. EESREHAB consisted of a combination of bipedal stepping on a treadmill with adjustable robotic body weight support (9 cm s−1, Robomedica) and overground quadrupedal walking supported in a multidirectional robotic body weight support interface24. EES was applied throughout the period of neurorehabilitation. Sessions lasted between 30 and 40 min.
Different experimental conditions used throughout the project are summarized in Fig. 2a. Mice were divided in three experimental groups: uninjured, SCI (no neurorehabilitation), and EESREHAB. At the end of the experimental period, mice were terminated to harvest fresh tissues or perfused and dissected. Half of the groups of mice underwent a terminal experimental condition immediately before being terminated, which is denoted by →final_condition. If more than one component was integrated in the terminal experimental condition, the additional component is denoted by ::. Group 1 (uninjured) consisted of uninjured mice that did not perform a terminal behavioural task. Mice in group 2 (SCI) received a contusion SCI and did not perform a terminal behavioural task. Mice in group 3 (EESREHAB) received a contusion SCI and followed EESREHAB for 4 weeks, but did not perform a terminal behavioural task. Mice in group 4 (SCI→EES::walking) received a contusion SCI and walked with EESON for 30 min immediately before being terminated. Mice in group 5 (EESREHAB→EES::walking) received a contusion SCI and followed EESREHAB for 4 weeks, and walked with EESON for 30 min immediately before being terminated. Mice in group 6 (EESREHAB→EES) received a contusion SCI and followed EESREHAB for 4 weeks, and were stimulated for 30 min with EES just below motor threshold immediately before being terminated. Mice in group 7 (EESREHAB→cortex) received a contusion SCI and followed EESREHAB for 4 weeks, and walked with optogenetic stimulation of the motor cortex for 30 min immediately before being terminated. Mice in group 8 (EESREHAB→cortex::walking) received a contusion SCI and followed EESREHAB for 4 weeks, and walked with EESON and optogenetic stimulation of the motor cortex for 30 min immediately before being terminated (see Supplementary Table 3).
All the behavioural procedures have been described in detail previously4,40. Locomotor performances of uninjured mice and mice with lateral hemisection SCI were evaluated during quadrupedal walking on a treadmill. Locomotor performances of mice with contusion SCI were evaluated during walking bipedally on a treadmill or during quadrupedal overground walking. All the final behavioural assessments of mice with contusion SCI were performed with EESOFF and repeated with EESON, but in the absence of 5-HT agonists. Bilateral leg kinematics were captured with twelve infrared cameras of a Vicon Motion Systems that tracked reflective markers attached to the crest, hip, knee, ankle joints and distal toes. The limbs were modelled as an interconnected chain of segments and a total of 80 gait parameters were calculated from the recordings. All gait parameters are reported in Supplementary Table 2. To evaluate differences between experimental conditions, as well as to identify the most relevant parameters to account for these differences, we implemented a multistep multifactorial analysis based on principal component analysis, which we described in detail previously28,61,62 (Extended Data Fig. 14). In brief, for each experiment dataset, the principal component analysis was performed by computing the covariance matrix A of the ensemble of parameters over the gait cycle, after subtraction of their respective mean values. The principal components were computed from eigenvalues λj and eigenvectors Uj of A. The principal components were ordered according to the amount of data variance accounted for by each component. The coordinate of each gait cycle on the first principal component—that is, the component vector explaining the greatest amount of variance across the gait parameters, was thereafter referred to as the walking performance.
Chronophotography was used to generate representative series of still pictures arranged in a single photograph to illustrate the locomotor abilities of mice. Videos at 25 fps or photographs at 15 fps were recorded while mice were performing locomotor tasks such as quadrupedal or bipedal walking on a treadmill or runway. Images from these recordings were chosen to best illustrate the different consecutive phases of walking of the hindlimbs−that is, stance and swing phases. The frequency of chosen pictures varied due to the varying velocity of the mice. The series of pictures were assembled in Photoshop while blending out non-essential detail.
Neuron-specific ablation and chemogenetics
For ablation experiments with the diphtheria toxin, AAV-flex-DTRV was infused in the lumbar spinal cord of Vsx2cre mice63. Four weeks after spinal infusions, mice received intraperitoneal injections of diphtheria toxin (Sigma, D0564) diluted in saline (100 µg kg−1) to ablate SCVsx2::Hoxa10 neurons. Mice were tested just before ablation and two weeks post-ablation. To manipulate the activity of SCVsx2::Hoxa10 neurons, AAV5-hSyn-DIO-hm4D or AAV5hSyn-DIO-hm3D64 were infused in the lumbar spinal cord of Vsx2cre mice four weeks prior to any behavioural experiments or SCI. On the day of the experiment, mice were tested on the behavioural task immediately before and between 30–45 min after intraperitoneal injections of 5 mg kg−1 clozapine N-oxide (CNO) (Carbosynth, CAS: 34233-69-7, suspended in 2% DMSO in saline)28. For chronic chemogenetic silencing, AAV5-hSynDIO-hm4D or AAV5-hSyn-DIO-hm3D was infused in the lumbar spinal cord of Vsx2cre mice four weeks prior to the SCI. Mice received approximately 0.05 mg ml−1 CNO with 5 mM sucrose65 in their drinking water each day, which amounted to approximately 5 mg kg−1 CNO per day. Experiments that involved chronic chemogenetic activation or silencing of SCVsx2::Hoxa10 neurons were performed two days after the CNO was removed from the drinking water.
Recording of muscle activity
A subset of mice that had EES electrodes implanted over the lumbar spinal cord were assessed with electrophysiology. Mice were anaesthetized with ketamine/xylazine. Ketamine maintenance doses were administered as needed. Two needle electrodes were inserted in the tibialis anterior muscle. Single-pulse stimulation of 200-µs-long pulses delivered every 5 s was applied to the dorsal surface of the spinal cord and muscle responses were recorded for 50 ms post-stimulation. The pulses (resulting in a stimulus artefact) were aligned to 0 ms, as shown in all figure panels (Extended Data Fig. 13). Stimulation consistently produced short-latency responses (likely to be monosynaptic responses) and long-latency responses (likely to be polysynaptic responses). We calculated the root mean squares followed by the integrals for 2–7 ms (early response) and 10–20 ms (long-latency response). Bar graphs report the long-latency muscle responses.
Mice were perfused at the end of the experiments. Mice were deeply anaesthetized by an intraperitoneal injection of 0.2 ml sodium pentobarbital (50 mg ml−1). Mice were transcardially perfused with PBS followed by 4% paraformaldehyde in PBS. Tissue was removed and post-fixed for 24 h in 4% paraformaldehyde before being transferred to PBS or cryoprotected in 30% sucrose in PBS.
Immunohistochemistry was performed as described previously28. Perfused post-mortem tissue was cryoprotected in 30% sucrose in PBS for 48 h before being embedded in cryomatrix (Tissue Tek O.C.T, Sakura Finetek) and freezing. Ten- or 20-micrometre-thick transverse sections of the spinal cord were cut on a cryostat (Leica), immediately mounted on glass slides and dried. Sections were blocked with 10% bovine serum albumin in PBS for 60 min. Then sections were incubated with the following primary antibody diluted in blocking solution at room temperature overnight: rabbit anti-GFAP (1:500, Dako Z0334), cFos (1:2,000 Synaptic Systems 226003), vGluT1 (1:1,000, Synaptic Systems 135302). Slides were washed four times with PBS before the secondary antibodies (Alexa Fluor Conjugated, ThermoFisher Scientific, USA) were applied for 90 min in blocking solution; donkey anti-rabbit Alexa Fluor 647 (1:1,000, A-31573), donkey anti-rat Alexa Fluor 647 (1:1,000, A-48272), donkey anti-goat Alexa Fluor 647 (1:1,000, A-21447). Slides were washed four times with PBS and then cover slipped with Mowiol. Immunofluorescence was imaged digitally using a slide scanner (Olympus VS-120 Slide scanner) or confocal microscope (Zeiss LSM880 + Airy fast module with ZEN 2 Black software (Zeiss)). Images were digitally processed using ImageJ (ImageJ NIH) software or Imaris (Bitplane, v.9.0.0).
The aim of the first set of experiments with the PRV Ba2017 was to optimize the timing required to achieve monosynaptic labelling of the brain after lumbar spinal cord infusions targeting the virus to Vsx2-positive neurons. Timepoints tested ranged from 1 day to 4 days using 12 h increments post-injection. Subsequently, a 3 day timepoint post-infusion was used for the remaining experiments. Post-mortem, brains were cut sagittally at 40 µm and directly mounted on glass slides. Every second section was imaged and imported into Neurolucida for brain reconstruction. Labelled neurons were counted per region.
Fluorescence in situ hybridization
To verify the location of cell types, to uncover the identity of cells that provide input to or receive connections from SCVsx2::Hoxa10 neurons, as well as to evaluate expression of activity-related genes in SCVsx2::Hoxa10 neurons, we performed in situ hybridization of cell-type markers and activity-related genes using RNAscope (Advanced Cell Diagnostics). Lists of putative marker genes were obtained from snRNA-seq data, as described below, and cross-referenced against a list of validated probes designed and provided by Advanced Cell Diagnostics. In total, probes were obtained for the following genes: Chat, catalogue (cat.) no. 408731; Maf, cat. no. 412951; Slc17a6, cat. no. 319171; Slc32a1, cat. no. 319191; Vsx2, cat. no. 438341; Pkd1l2, cat. no. 520211; Tac2, cat. no. 446391. We then generated 12-µm cryosections from fixed-frozen spinal cords as previously described66 and performed fluorescence in situ hybridization for each probe according to the manufacturer’s instructions, using the RNAscope Fluorescent Multiplex Reagent Kit (cat. no. 323133) or HiPlex kit (cat. no. 324106).
Samples were incubated in X-CLARITY hydrogel solution67,68 (Logos Biosystems) for 24 h at 4 °C with gentle shaking. Samples were degassed and polymerized using the X-CLARITY Polymerisation System (Logos Biosystems). Samples were washed in 0.001 M PBS for 5 min at room temperature then placed in the X-CLARITY Tissue Clearing System (Logos Biosystems), set to 1.5 A, 100 RPM, 37 °C, for 29 h. Clearing solution was made in house with 4% sodium dodecyl sulfate (SDS), 200 mM boric acid with dH20, pH adjusted to 8.5. The samples were washed for at least 24 h at room temperature with gentle shaking in 0.1 M PBS solution containing 0.1% Triton X-100 to remove excess SDS. The samples were incubated in 40 g of Histodenz dissolved in 30 ml of 0.02 M PB, pH 7.5, 0.01% sodium azide (refractive index 1.465) for at least 24 h at room temperature with gentle shaking prior to imaging.
Mice underwent a final EESREHAB session and were perfused69,70 60 min later with 0.1 M PBS followed by 4% PFA (in 0.1 M PBS). Samples were dissected and post-fixed in 4% PFA (in 0.1 M PBS) at 4 °C overnight and placed in 0.1 M PBS containing 0.03% sodium azide. Immunolabelling of the samples was performed by first pretreating with methanol in 2 ml Eppendorf tubes by dehydrating with a methanol/H2O series at 1 h each at room temperature with shaking at 60 RPM: 20%, 40%, 60%, 80% and 100%. This procedure was followed by 1 h washing with 100% methanol before chilling the samples at 4 °C. Samples were then incubated overnight with shaking in 66% dicholoromethane/33% methanol at room temperature. The samples were washed twice in 100% methanol with shaking at room temperature and then bleached in chilled fresh 5% H2O2 in methanol overnight at 4 °C. Samples were rehydrated with a methanol/H2O series: 80%, 60%, 40%, 20% and 0.1M PBS, each for 1 h at room temperature under shaking. Samples were washed for 1 h × 2 at room temperature in PTx.2 buffer (0.1 M PBS with 0.2% Triton X-100) under shaking. This was followed by an incubation in 2 ml of permeabilization solution (400 ml PTx.2, 11.5 g glycine, 100 ml DMSO for a total stock volume of 500 ml) for 2 days at 37 °C with shaking at 60 RPM. Samples were incubated in 2 ml of blocking solution (42 ml PTx.2, 3 ml of normal donkey serum, 5 ml of DMSO for a total stock volume of 50 ml) for 2 days at 37 °C with shaking. The samples were incubated for 7 days at 37 °C with shaking in primary antibody solution consisting of PTwH (0.1 M PBS, 2 ml Tween-20, 10 mg l−1 heparin, 5% dimethyl sulfoxide, 3% normal donkey serum), and cFos antibody (1:2,000, Synaptic Systems, 226003) for a total volume of 2 ml per sample. Samples were washed in PTwH for 24 h with shaking and incubated for 7 days at 37 °C with shaking in secondary antibody solution consisting of PTwH, 3% normal donkey serum and donkey anti-rabbit Alexa Fluor 647 (1:400, ThermoFisher Scientific) in a total volume of 2 ml per sample. Samples were washed in PTwH for 24 h with shaking at room temperature. Clearing of the samples was performed by first dehydrating the samples in a methanol/H2O series as follows: 20%, 40%, 60%, 80% and 100% twice each for 1 h with shaking at room temperature followed by a 3 h incubation with shaking in 66% dichloromethane/33% methanol at room temperature. Samples were incubated in 100% dichloromethane 15 min twice with shaking to wash residual methanol. Finally, samples were incubated in 100% dibenzyl ether without shaking for refractive index matching of the solution for at least 24 h prior to imaging.
uDISCO71 clearing of the mouse spinal cord was initiated by stepwise dehydration in increasing concentrations of tert-butanol diluted in dH2O with a total volume of 5 ml at 35 °C as follows: 30% tert-butanol overnight, 50% for 10 h, 70% overnight, 80% for 10 h, 90% overnight, 96% for 10 h and 100% overnight. The samples were then incubated in 5 ml of dichloromethane at room temperature for 70 min with shaking. This was then followed by incubation in BABB-D4 (BABB: 2:1 mixture of benzyl benzoate to benzyl alcohol; 4:1 mixture of BABB to diphenyl ether; 0.4% volumes vitamin E) for 24 h at room temperature shaking at 60 RPM prior to imaging.
Imaging of cleared tissue was performed using a customized MesoSPIM and CLARITY- optimized light-sheet microscope (COLM), as described23,72. A custom-built sample holder was used to secure the central nervous system in a chamber filled with RIMS. Samples were imaged using either a 1.25× or 2.5× objective at the mesoSPIM72 and a 4× or 10× objective at the COLM23 with one or two light sheets illuminating the sample from the left and right sides. The voxel resolution in the x, y and z directions was 5.3 µm × 5.3 µm × 5 µm for the 1.25× acquisition and 2.6 µm × 2.6 µm × 3 µm for the 2.5× acquisition. The voxel resolution of the COLM was 1.4 µm × 1.4 µm by 5 um for the 4× and 0.59 µm × 0.59 µm × 3 µm for the 10× acquisition. Images were generated as 16-bit TIFF files and then stitched using Arivis Vision4D (Arivis). 3D reconstructions and optical sections of raw images were generated using Imaris (Bitplane, V.9.0.2) software.
cFos positive neurons of cleared samples were quantified using Arivis Vision4D (Arivis). After defining a region of interest around the grey matter, each sample was subjected to a custom-made pipeline. We applied morphology, denoising, and normalization filters to enhance the signal of bright objects and homogenized the background. Threshold-based segmentation of the cFos signal was applied within predefined 3D regions to quantify the total number of cFos positive cells. Image analysis parameters were kept constant among all samples.
Neuron-specific recordings and analysis
AAV5-Syn-flex-Chrimson was infused in the lumbar spinal cord of Vsx2cre mice at least four weeks prior to terminal experiments. Mice were anaesthetized with ketamine/xylazine. Ketamine maintenance doses were then administered as needed. Four-shank, multi-site electrode arrays (NeuroNexus A4x16-Poly2-5 mm-23s-200-177) were lowered into the spinal cord to a depth of 800 µm, with shanks arranged longitudinally at 350 µm from midline. Signals were recorded with a NeuroNexus Smartbox Pro using a common average reference and while applying 50 Hz notch and 450–5,000 Hz bandpass filters. Stimulation was controlled with a Multi-Channel Systems STG 4004 and MC_Stimulus II software. ChrimsonR-expressing neurons were identified using optogenetic stimulation. Ten pulse trains of 1-ms pulses were delivered at 20 Hz from a 635 nm laser (LaserGlow Technologies LRD-0635-PFR-00100-03). Laser light was delivered to the surface of the spinal cord through a fibre optic cable attached to 400 µm, 0.39 NA cannula with a 5 mm tip (Thorlabs). Optical power was set to 2.35 mW at the tip. Electrical stimulation (EES and reticular formation) consisted of 200–µs pulses delivered every 5 s. EES was delivered with a micro fork probe (Inomed, 45 mm straight, item no. 522610) positioned along the midline just caudal to the recording array. Stimulation of the reticular formation was delivered with a platinum/iridium bipolar concentric electrode (Microprobes PI-SNE-100) placed at −5.8 mm caudal and 0.3 lateral from Bregma, 5.6 mm deep from the brain surface. Spike sorting was performed with SpyKING CIRCUS v.1.0.773. The median-based average electrical stimulation artefacts for each channel were subtracted from the recordings prior to sorting. Due to the size and variability of the artefacts, periods containing residual stimulation artefacts were not sorted (–1.0 to +1.5 ms and +2.5 ms around stimulus onset for EES and reticular formation stimulation onset, respectively). Sorting results were manually curated using Phy (https://github.com/cortex-lab/phy). Single unit clusters were selected for analysis based on their biphasic waveforms and template amplitudes above 50 µV, as well as strong refractory period dips in their spike autocorrelograms. Similar clusters were merged according to the Phy manual clustering guide. ChrimsonR-expressing, putative SCVsx2::Hoxa10 neurons were identified based on their low-latency and lowjitter responses to light pulses. Specifically, a one-sided Wilcoxon signed-rank test was used to compare the instantaneous firing rate of units 10 ms before stimulus onset and 6 ms after. Those neurons with a post-stimulus onset firing rate increase of P value less than 0.001 and response jitter (standard deviation of latency) less than 2 ms were considered to be directly activated and therefore SCVsx2::Hoxa10 neurons that displayed early responses to electrical stimulation (EES or reticular formation), indicative of putative monosynaptic inputs, were identified using the same firing rate test in addition to a jitter of less than 1.2 ms and minimum spike probability in the first 6 ms after stimulation greater than 20%. For stimulation of the reticular formation, the post-stimulus onset quantification window was increased to 7 ms to account for conduction time from the brainstem to the spinal cord74.
Fabrication of optoelectronic implants integrating microLEDs and EES
The fabrication of the micro-LED array was based on a previously validated technological design40 that we adapted to incorporate electrodes to deliver EES, as illustrated in Extended Data Fig. 15a. A 4-inch silicon wafer coated with Ti/Al (25/100 nm) was spin-coated with a 3 mm thick polyimide layer (PI2610, HD Microsystems), followed by a curing process of 2 h at 300 °C in a N2 oven. A Ti/Au/Ti metal layer (25/250/25 nm) was sputtered after O2 plasma surface activation (AC450, Alliance Concept). Wet etching for Au and reactive ion etching (RIE) for Ti patterned the metal layer after the photolithography (AZ1512, MicroChemicals). A polyimide layer (2-µm thick) was then spin-coated and cured to encapsulate the patterned metallization layer. Photolithography (AZ9620, MicroChemicals) and RIE etching patterned the polyimide-metal-polyimide stack. Next, A 20-nm-thick SiO2 layer was sputtered and followed by the spin-coating of a 15–µm-thick polydimethylsiloxane (PDMS) (Sylgard 184, Dow Corning) after O2 plasma surface activation. RIE etching of the PDMS layer after the photolithography (AZ40XT, MicroChemicals) exposed openings for the micro-LED integration sites and electrical stimulation sites. For the micro-LED integration, the solder paste (diameter 50 mm, SMDLTLFP10T5, Chipquik) and blue microLEDs (TR2227, Cree) were deposited onto the contact pads using a pick-and-place equipment (JFP Microtechnic). The microLEDs were bonded through the solder paste reflow at 165 °C and the exposed connection areas around microLEDs were drop-cast with a 14 wt% solution of polyisobutylene (PIB, Oppanol, BASF) in cyclohexane (Sigma-Aldrich). After solvent evaporation (10 min at 55 °C), the device was cured for 4 h at room temperature. Next, a 50 wt % PDMS-phosphor composite (HTR620, PhosphorTech) was deposited over the PIB-encapsulated blue microLEDs via pneumatic printing to activate red-shifted opsins. Electrical stimulation sites were coated after O2 plasma surface activation with a platinum-silicone composite comprised of 100 µg of platinum microparticle powder (Goodfellow) mixed into a 110 ml PDMS/cyclohexane solution (200 mg/500 ml, Dow Corning, Sigma-Aldrich). The mixture turned into a paste after the cyclohexane evaporation, and the paste was placed onto a laser-cut PET mask to selectively fill openings via screen printing. After the PET mask removal, the device was cured overnight at room temperature, followed by 4 h at 55 °C. A 50–µm-thick PDMS layer was manually spread on the surface of the implant except for the conductive composite sites (~70 mm) for ease of handling during the surgical process. Stainless steel wires from a circular connector (A71914/A71915, Omnetics) were soldered onto the implant pads and sealed with silicone (734, Dow Corning). As a last step, the implant was released from the wafer through anodic dissolution of the Al layer at 1.2 V bias in a NaCl-saturated deionized water.
Implantation of the optoelectronic implant
Procedures have been described in detail previously40. In brief, the interlaminar spaces between vertebrae T12/T13 and L2/L3 were dissected to expose the exit and entry points, respectively, for the implant. A 6-0 ethilon suture (MPE697H, Ethicon EMEA) was passed through the epidural space from T12/T13 to L2/L3, then through the silicone loop of the implant and back through the epidural space. The implant was slid over the spinal cord by gently pulling both ends of the suture rostrally. The connector of the implant was fixed by suturing paraspinal muscles across the connector. The percutaneous connector (16-pin connector, A79112-001, Omnetics Connector Corporation) and wires were routed subcutaneously to the head. Three screws (part no. AMS120/5B-25, Antrin miniature specialties) were inserted into the skull, surrounding the percutaneous connector. Fresh dental cement was then poured around the screws and connector, and held in place until cured. Photostimulation protocols for inhibition of SCVsx2::Hoxa10 consisted of 20 ms pulses at 50 Hz (100% duty cycle).
Behavioural assays were replicated 3 to 10 times depending on the experiments and averaged per animal. Statistical analysis was performed in R (version 3.6.3). Two-sided paired or independent t-tests, one-way ANOVA or two-way repeated measures ANOVA were used as appropriate, followed by post hoc significance testing. Alpha was set as 0.05. Non-parametric Mann–Whitney or Wilcoxon signed-rank tests were used when comparisons involved fewer than five mice. Representative experiments such as histological micrographs were repeated in a minimum of four mice.
Single-nucleus RNA sequencing
We performed single-nucleus dissociation of the mouse lumbar spinal cord according to our previously described procedures9,12. Following euthanasia by isoflurane inhalation and cervical dislocation, the lumbar spinal cord site was immediately dissected and frozen on dry ice. We denounced spinal cords in 500 µl sucrose buffer (0.32 M sucrose, 10 mM HEPES pH 8.0, 5 mM CaCl2, 3 mM magnesium acetate, 0.1 mM EDTA, 1 mM DTT) and 0.1% Triton X-100 with the Kontes Dounce Tissue Grinder. Two millilitres of sucrose buffer was then added and filtered through a micrometre cell strainer. The lysate was centrifuged at 3,200 g for 10 min at 4 °C. The supernatant was decanted, and 3 ml of sucrose buffer was added to the pellet and incubated for 1 min. The pellet was homogenized using an Ultra-Turrax and 12.5 ml density buffer (1 M sucrose, 10 mM HEPES pH 8.0, 3 mM Mg acetate, 1 mM DTT) was added below the nuclei layer. The tube was centrifuged at 3,200 g at 4 °C and supernatant poured off. Nuclei on the bottom half of the tube wall were collected with 100 µl PBS with 0.04% BSA and 0.2 U µl−1 RNase inhibitor. Resuspended nuclei were filtered through a 30–µm strainer, and adjusted to 1,000 nuclei per µl.
We carried out snRNA-seq library preparation using the 10x Genomics Chromium Single Cell Kit version 2. The nuclei suspension was added to the Chromium RT mix to achieve loading numbers of 5,000. For downstream cDNA synthesis (13 PCR cycles), library preparation and sequencing, the manufacturer’s instructions were followed.
Reads were aligned to the most recent Ensembl release (GRCm38.93) using Cell Ranger, and a matrix of UMI counts, including both intronic and exonic reads, was obtained using velocyto75. Seurat30 was used to calculate quality control metrics for each cell barcode, including the number of genes detected, number of UMIs, and proportion of reads aligned to mitochondrial genes. Low-quality cells were filtered by removing cells expressing less than 200 genes or with more than 5% mitochondrial reads. Genes expressed in less than three cells were likewise removed, yielding a count matrix consisting of 22,806 genes in 81,657 cells.
Clustering and integration
Prior to clustering analysis, we first performed batch effect correction and data integration across the two different experimental conditions as previously described30. Gene-expression data was normalized using regularized negative binomial models76, then integrated across batches using the data integration workflow within Seurat. The normalized and integrated gene expression matrices were then subjected to clustering to identify cell types in the integrated dataset, again using the default Seurat workflow. Cell types were manually annotated on the basis of marker gene expression, guided by previous studies of the mouse spinal cord9,12,31,32.
RNA velocity was calculated using the velocyto package75. Velocyto estimates cell velocities from their spliced and unspliced mRNA content. We generated the annotated spliced and unspliced reads using the run10x function of the Velocyto command line tool. We then calculated gene-relative velocity using k-nearest neighbour pooling with k = 10 (default), quantile = 0.1 (default). For snRNA-seq, we set emat to 0.006 and nmat to 0.004. For spatial transcriptomics, we set emat to 0.01 and nmat to 0.01.
The lumbar spinal cords of mice were embedded in OCT and cryosections were generated at 10 µm at –20 °C. Sections were immediately placed on chilled Visium Tissue Optimization Slides (cat. no. 1000193, 10x Genomics) or Visium Spatial Gene Expression Slides (cat. no. 1000184, 10x Genomics). Tissue sections were then fixed in chilled methanol and stained according to the Visium Spatial Gene Expression User Guide (cat. no. CG000239 Rev A, 10x Genomics) or Visium Spatial Tissue Optimization User Guide (cat. no. CG000238 Rev A, 10x Genomics). For gene-expression samples, tissue was permeabilized for 12 min, which was selected as the optimal time based on tissue-optimization time-course experiments. Bright-field histology images were taken using a 10× objective on a slide scanner (Olympus VS-120 Slide scanner). For tissue-optimization experiments, fluorescent images were taken with a TRITC filter using a 10× objective and 400 ms exposure time.
Spatial transcriptomics libraries were prepared according to the Visium Spatial Gene Expression User Guide. They were then clustered at 270 pM on a paired-end HiSeq4000 flow cell and sequenced on a HiSeq4000 System (Illumina) at a sequencing depth of approximately 140–180 million reads per sample. Sequencing was performed using the following read protocol: read 1: 28 cycles; i7 index read: 8 cycles; i5 index read: 8 cycles; and read 2: 98 cycles.
Raw FASTQ files and histology images were processed using the Space Ranger software (version 1.0.0). Reads were aligned to the most recent Ensembl release (GRCm38.93), and a matrix of UMI counts, including both intronic and exonic reads, was obtained using velocyto75. Seurat30 was used to calculate quality control metrics for each cell barcode, including the number of genes detected, number of UMIs, and proportion of reads aligned to mitochondrial genes. Low-quality barcodes were filtered by removing cells expressing less than 5,000 UMIs. Genes expressed in less than 3 barcodes were likewise removed, yielding a UMI count matrix consisting of 22,127 genes and 9,755 barcodes across 61 spinal cord sections from 12 mice from four experimental conditions. To align all sections to a common coordinate space, we implemented a custom image analysis pipeline that includes preprocessing, registration and combination of histological images from different sections. In brief, we implemented all preprocessing in Fiji, and all registration procedures in R, using the image analysis package imageR, and medical image registration package RNiftyReg. Images were aligned to the L3 spinal cord segment from a standard histological atlas. Regions were assigned on the basis of their location within the cytoarchitecture of the spinal segment.
Cell type deconvolution
To integrate our spatial and single-nucleus transcriptomes, we used robust cell type decomposition77 (RCTD) to localize each neuronal subpopulation inferred from snRNA-seq data within the mouse spinal cord. In brief, RCTD deconvolves each spatial barcode into a mixture of one or more neuronal subpopulations, while accounting for technical differences between single-nucleus and spatial transcriptomes. RCTD was run with doublet mode disabled, allowing each barcode to potentially contain more than two cell types, to produce a matrix of 9,755 spatial barcodes by 36 neuronal subpopulations. The cells in this matrix represented the neuronal subpopulation or subpopulations inferred at each spatial barcode. We observed spatial distributions that were largely compatible with existing knowledge about the locations of each neuronal subtype within the spinal cord, notwithstanding some minor discrepancies, which can likely be attributed to the relatively large regions captured by each spatial barcode, the depth of our snRNA-seq data, and the higher degree of transcriptional similarity between ventral neuronal subpopulations in the spinal cord. We visualized the spatial distribution of neuronal subpopulations by plotting the scores assigned for each subpopulation within the common coordinate system of the registered spinal cord. We recovered smoothed patterns of spatial deconvolution with two-dimensional locally weighted regression, as described by the authors of RCTD77. In addition, we computed the mean RCTD score for each neuronal subpopulation in each of the five spinal cord regions assigned by the Allen Brain Atlas.
To identify genes differentially expressed in SCVsx2::Hoxa10 neurons, we performed differential expression testing within each comparison using negative binomial generalized linear mixed models (GLMMs), as previously described78 and as implemented in the Libra R package, available at https://github.com/neurorestore/Libra. We incorporated library size factors as an offset term, and calculated statistical significance using a likelihood ratio test against a reduced model. We focused our analysis on VE-1 neurons, as these were prioritized by Augur with the highest median AUC across all six comparisons. To further dissect the significance of the observed transcriptional changes in response to perturbations on different timescales, we then divided the six comparisons into groups of acute and chronic perturbations. The chronic perturbations consisted of EESREHAB versus SCI and EESREHAB→EES::walking versus SCI→EES::walking; the remaining perturbations were considered to be acute perturbations. We tested for enrichment of immediate early genes, using a list of genes manually curated by Hrvatin et al.79, by applying fgsea80 to the signed −log10P values estimated by the GLMMs, and compared the normalized enrichment scores estimated by fgsea between acute and chronic perturbations. To identify genes specifically upregulated in chronic perturbations, we performed a one-sided t-test on the coefficients estimated by the GLMMs, limiting our analysis to genes for which the GLMMs could be fit in all six comparisons.
Cell type prioritization with Augur
To identify neuronal subpopulations activated by key therapeutic features of EESREHAB, we developed a machine learning method that we named Augur12,13. The key assumption underlying Augur is that cell types undergoing a profound response to a perturbation should become more separable, within the highly multidimensional space of gene expression, than less affected cell types. To quantify this separability, we framed this problem as a classification task. In brief, Augur withholds a proportion of sample labels, then trains a random forest classifier to predict the condition from which each cell was obtained (for instance, diseased or healthy tissue). The accuracy with which this prediction can be made from single-cell gene expression measurements is then evaluated in cross-validation, and quantified using the area under the receiver operating characteristic curve (AUC). This process is repeated separately for each cell type, such that the AUC provides a quantitative measure of separability that can be used to rank cell types based on the relative magnitude of their response to an arbitrary perturbation. We refer to this process as cell type prioritization.
To identify the neuronal subpopulations engaged by EESREHAB, we applied Augur to six key comparisons involving the eight experimental groups. Five of these six comparisons involved acute perturbations on the timescale of transcription (minutes to hours), raising a risk that the total transcriptional output of each cell may not yet fully reflect the impact of the perturbation at the time of snRNA-seq12. Consequently, for these five comparisons, we applied Augur to a matrix of RNA velocity75, as previously described12,13,75. For the remaining comparison (EESREHAB vs SCI), Augur was applied directly to the UMI count matrix. Augur was run with default parameters for all comparisons. To evaluate the robustness of cell type prioritizations to the resolution at which neuronal subpopulations were defined in the snRNA-seq data, we applied Augur at various clustering resolutions, and visualized the resulting cell type prioritizations both on a hierarchical clustering tree81 of neuron subpopulations and as a progression of UMAPs.
Spatial prioritization with Magellan
To enable spatial prioritization of the perturbation response within complex tissues, we developed Magellan. Magellan builds on the concept of transcriptional separability that provides a basis for cell type prioritization in Augur. However, in spatial transcriptomics data, the analytical level of interest is not necessarily a cell type, but rather a location within a two- or three-dimensional tissue. To approach the data at this level, we sought to evaluate the transcriptional separability between barcodes from two experimental conditions at each point within a common coordinate system. We reasoned that we could achieve this by evaluating the separability of barcodes from each condition within small, overlapping tiles, layered across the spatial coordinate system. In brief, for each barcode in a spatial transcriptomics dataset, Magellan selects the k-nearest neighbours from each experimental condition within common coordinate space, where k is set to 20 by default. Then, Magellan withholds the experimental condition labels for a proportion of these neighbours, and trains a random forest classifier to predict the experimental condition given the remaining barcodes as input. The accuracy of these predictions is evaluated in the withheld barcodes, and the process is repeated in three-fold cross-validation. As in Augur, the accuracy is quantified using the AUC. The cross-validation is repeated several times (by default, 50 times) in order to converge at a robust estimate of the AUC. The entire procedure is repeated for each barcode in the dataset, providing a spatial map of the AUC over the coordinate system of the spatial transcriptomes.
We then generated simulated data to validate Magellan. We devised a sequence of spatial patterns that we reasoned would capture key desiderata of a spatial prioritization method. Our premise was that an ideal method would be capable of detecting both sharp borders and smooth gradients, and would be capable of resolving quantitative differences between different aspects of a multifaceted perturbation response. We used Splatter82 to simulate spatial transcriptomics data for six patterns that captured this premise. Simulation parameters were estimated from our own spatial transcriptomics dataset using the splatEstimate function. A total of 5,000 barcodes were simulated for each pattern, and arranged within the common coordinate system of the mouse lumbar spinal cord. A fixed proportion of 10% of all genes in the dataset were set to be differentially expressed between the two simulated conditions (using the de.prob parameter), with the intensity of the differential expression varying according to the simulated spatial pattern (controlled with the de.facLoc parameter). Magellan was applied to each simulated dataset with default parameters, with two exceptions. First, cross-validation was repeated 100 times for each barcode in order to estimate the number of repeated cross-validation folds required to obtain a robust estimate, which was achieved by comparing the AUC assigned to each barcode in the first 50 samples to the second 50 samples. Second, to evaluate the effect of the parameter k, we ran Magellan with k = 20, 50 or 100 neighbours for each spatial barcode.
We implemented Magellan as an R package, available from https://github.com/neurorestore/Magellan. Magellan builds on Augur by reusing its procedures for feature selection, classification, and cross-validation. However, unlike Augur, Magellan requires as input a spatial transcriptomics dataset in which each barcode is associated with a two-dimensional coordinate and an experimental condition.
To enable spatial prioritization in our own dataset, we applied Magellan to four key comparisons between four experimental conditions. Barcodes from the white matter were excluded, and two low-quality sections excluded (Slide1_4_B1_M3_6wNT, Slide1_2_B3_M10_6wNT). In view of the left-right symmetry of the spinal cord, we replaced the coordinate of each barcode on the x-axis with its absolute value in order to mitigate artefacts introduced by the registration procedure. Magellan was run with default parameters (k = 20) and with k = 50 or 100 in order to illustrate the effect of spatial resolution on our results. We used an identical local regression procedure to that described above for spatial deconvolution with RCTD to visualize smoothed spatial prioritizations77.
Embedding single-nucleus transcriptomes in space
To corroborate the spatial prioritizations assigned by Magellan, we leveraged Tangram36 to embed single-nucleus transcriptomes within the common coordinate system of the mouse spinal cord. We aligned single-cell barcodes from each of the four matching experimental conditions to the corresponding spatial transcriptomics data, using 100 marker genes and training the model for 100 epochs. Spatial barcodes from the white matter were excluded from this analysis. This procedure assigned a spatial coordinate to each single-nucleus transcriptome. We then correlated the AUCs assigned by Augur to each single-nucleus transcriptome to the AUCs assigned by Magellan at the matching spatial coordinates. Finally, to approximate the degree of concordance between cell type and spatial prioritizations, we computed the mean AUC for all spatial barcodes overlapping with single-nucleus transcriptomes of a given cell type.
We performed computer simulations on a previously validated spiking neural network model37,38, reproducing the proprioceptive feedback circuits associated with a pair of antagonist muscles in the lumbar spinal cord of rodents. Computer simulations were performed in Python 2.7 using the NEURON simulation environment83.
The spiking neural network includes populations of group Ia and group II afferent fibres, Ia inhibitory interneurons, group II excitatory interneurons, and pools of alpha motor neurons. The number of cells, the number and the strength of the synapses contacting the different populations of neurons, and the characteristics of the cell models are described in our previous work37,38.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
#neurons #restore #walking #paralysis