Abstract
Historically, the membrane attack complex, composed of complement components C5b-9, has been connected to lytic cell death and implicated in secondary injury after a CNS insult. However, studies to date have utilized either non-littermate control rat models, or mouse models that lack significant C5b-9 activity. To investigate what role C5b-9 plays in spinal cord injury and recovery, we generated littermate PVG C6 wildtype and deficient rats and tested functional and histological recovery after moderate contusion injury using the Infinite Horizon Impactor. We compare the effect of C6 deficiency on recovery of locomotor function and histological injury parameters in PVG rats under two conditions: (1) animals maintained as separate C6 WT and C6-D homozygous colonies; and (2) establishment of a heterozygous colony to generate C6 WT and C6-D littermate controls. The results suggest that maintenance of separate homozygous colonies is inadequate for testing the effect of C6 deficiency on locomotor and histological recovery after SCI, and highlight the importance of using littermate controls in studies involving genetic manipulation of the complement cascade.
Subject terms: Complement cascade, Spinal cord diseases
Introduction
Traumatic spinal cord injury (SCI) causes a series of secondary degenerative events thought to exacerbate injury pathology1–3. One component of secondary injury after SCI is activation of the classical and alternative pathways of the complement cascade1,4. The complement cascade is composed of more than 30 soluble and membrane-bound proteins. The classical and alternative pathways converge on the terminal complement pathway, leading to the assembly of a multimeric protein complex, C5b-9, for which C6 is a necessary component5,6.
Previous studies suggest a detrimental role for C6/C5b-9 and activation of the terminal complement pathway in Central Nervous System (CNS) injury and disease. C5b-9 formation is thought to impede functional recovery and exacerbate pathology after CNS trauma7–12. CNS cells, particularly neurons and oligodendrocytes, are highly susceptible to C5b-9-mediated cell death in vitro13–17. In accordance with this observation, these cells express low levels of CD59, a membrane bound inhibitor of C5b-9 formation18, and deletion of CD59 increases C9 deposition in the injured spinal cord in association with increased histopathological inflammation, injury and demyelination compared to WT mice11. Moreover, C5b-9 is implicated in demyelination in experimental allergic encephalomyelitis (EAE)8,19, and demyelination-related Wallerian degeneration in peripheral nerve injury10. C5b-9 is also implicated as a mediator of tissue damage in atherosclerosis20–22, rheumatoid arthritis23,24, Alzheimer’s disease25,26, Huntington’s disease27, and Pick’s disease28.
In contrast, some evidence suggests that C5b-9 formation can result in not only cell lysis, but modulation of cell signaling when formed at sub-lytic levels. Sublytic C5b-9 induces polymorphonuclear leukocytes to produce reactive oxygen metabolites29 and increase endothelial synthesis of IL-8 and MCP-130. In nervous system cells, sublytic C5b-9 induces Schwann cell proliferation31,32, stimulates oligodendrocyte proliferation, and enhances oligodendrocyte survival33–37. Taken together, these data suggest divergent or multiple roles for C6 and C5b-9 assembly in inflammation and CNS injury.
To investigate the role of C6 in SCI, we initially acquired Piebald-Viral Glaxo (PVG) C6-deficient (C6-D) rats from the University of Wales and PVG WT rats from Harlan laboratories. PVG C6-D rats carry a spontaneous mutation resulting in a lack of the C6 protein and are incapable of C5b-9 formation2,9. While heterozygous colony breeding to generate littermate controls for mouse transgenic studies is the standard for the field, this approach is not commonly applied for comparison of C6 deficiency in PVG rats. A literature search identifying papers that employed C6 WT and C6-D rats identified 48 studies. 28 studies utilized the C6-D PVG strain for xenograft or in vitro research and 2 describe characterizations of the C6 deficiency. Focusing on the 18 studies that used the C6-D PVG strain for investigation of experimental injury or disease, none detail the use of a littermate paradigm under the experimental methods. While animal source/breeding paradigm cannot be definitively determined due to lack of detail in some (5), the majority (13) report maintenance of C6-D and WT rats as separate colonies, or that the C6D and WT rats employed were ordered from separate companies. A further breakdown of these 18 studies reveals studies in each of the following disease/trauma models: infection38, experimental autoimmune neuritis39, lung inflammation40, arthritis41 experimental diabetes42, seizure43, experimental SCI10, the EAE model8, nephropathy44, kidney damage45, renal disease46, renal microvascular injury47, experimental nephrotic syndrome48, and 5 studies on nephritis49–53. The results reported here compare the effect of C6 deficiency on recovery of locomotor function and histological injury parameters in PVG rats under two conditions: (1) animals maintained as separate C6 WT and C6-D homozygous colonies; and (2) establishment of a heterozygous colony to generate C6 WT and C6-D littermate controls.
Results
Confirmation of C6-deficiency
A PCR genotyping protocol was established for C6 deficiency by blast identification of a novel restriction site susceptible to Ava I cleavage and development of primer sequences enabling identification of restriction fragment lengths that could distinguish WT, heterozygous, and C6-D genotypes, as described under methods. In this protocol, WT (C6+/+) DNA is not cut and runs as a single band of ~ 200 bp, heterozygous (C6+/−) DNA exhibits incomplete digestion with two bands at ~ 150, and 200 bp, and homozygous C6D (C6−/−) DNA exhibits complete digestion with one band at ~ 150 bp (Fig. 1b). The genotyping protocol was validated using rats sourced from homozygous and heterozygous breeding colonies, and by comparison with CH50 assay for dose-dependent lysis of IgG sensitized sheep erythrocytes (Fig. 1a). To further confirm that C5b-9 was present only in F2-C6-WT animals and not in F2-C6-D animals immunohistochemistry using an anti-C5b-9 antibody was conducted54,55. C5b-9 was observed only in the gray and white matter of F2-C6-WT SCI animals, and not in either F2-C6-D animals or sections for which the primary was omitted (Fig. 2).
C6 deficiency impairs locomotor function in F2-C6 PVG rats but not H-C6 PVG rats
For our initial experiment, rats were maintained as separate homozygous colonies as previously reported by many investigators (H-WT or H-C6-D PVG; homozygous colony cohort). In a subsequent experiment, we generated experimental animals from F2 crosses to yield littermate controls (F2-WT and F2-C6-D PVG; littermate control cohort). Animals from both cohorts received SCI at 4–6 months of age and were within 10% variation in weight (range 169.2–195.8 g). Multiple tasks were used to assess functional locomotor recovery after SCI. BBB is an open-field locomotor test that assesses gross functional improvements such as stepping and coordination. The higher a BBB score, the more functional the animal. Analysis in the homozygous colony cohort showed that on average, H-C6-D rats exhibited improved outcome vs. H-WT rats, as seen by higher BBB scores, suggesting that C6 deficiency improved locomotor outcome (Fig. 3a; WT: filled black squares, H-C6-D: open black squares; two way ANOVA p < 0.05, Bonferroni’s multiple comparisons Day 42 < 0.05). In contrast, this result was reversed when littermate controls were used: F2-C6-D rats exhibited impaired locomotor outcome, measured by lower BBB scores, vs. F2-WT rats (Fig. 3b; WT: filled blue squares; F2-C6-D open blue squares; two way ANOVA Genotype p = 0.0006, Bonferroni’s multiple comparisons Day 42 post-hoc Day 42 p < 0.01). Horizontal ladder beam analysis was consistent with these BBB results. Ladderbeam is a quantitative measure that assesses the number of errors made by the animal as it traverses a 20-rung horizontal ladder. Thus, the higher the number of errors, the less functional the animal. In the homozygous strain cohort, H-C6-D animals exhibited a decrease in average ladder beam errors vs. H-WT animals (Fig. 3c; WT: filled black bars, H-C6-D: open black bars; Student’s t test p < 0.05), consistent with improved recovery of function. Conversely, in the littermate control cohort, F2-C6-D rats showed no improvement, and a strong trend for an increase in errors vs. F2-WT rats (Fig. 3d; WT: filled blue bars; F2-C6-D open blue bars; Student’s t test p = 0.09).
Variation in behavioral recovery kinetics and plateau was observed across these sequential studies, with WT littermate control cohort animals performing significantly better than WT homozygous colony animals in BBB and worse in horizontal ladder beam testing. While this could suggest that homozygous colony and littermate control WT rats responded differently to SCI, these cohorts were injured more than 2 years apart, and could therefore have been affected by variables that cannot be excluded. For this reason, a conservative data analysis approach was taken, and no statistical comparisons between cohorts are made in these figures.
Horizontal ladder beam is most sensitive to recovery of function after SCI in the range of stepping recovery56. Because of the high performance plateau in the littermate cohort, we employed a supplemental assessment, Catwalk kinematic analysis, to assess fine parameters of gait after SCI in addition to stepping function (Fig. 4). Data were normalized to pre-injury data (dashed lines). One-sample t tests were used to compare baseline (dashed line) and post-injury performance; the closer the group mean is to baseline the better recovery post-SCI. Using this analysis, F2-C6-D rats consistently exhibited group means that showed decrements in recovery in comparison with WT animals. Both F2-C6 WT and F2-C6-D rats exhibited a significant decrease in print area, indicative of weight bearing, the higher the number, the more weight bearing, from pre-injury baseline (Fig. 4a, one sample t test #p < 0.05), suggesting less weight support; however, F2-C6-D rats exhibited a significant further decrement in comparison with F2-C6-WT (Fig. 4a, Student’s t test *p = 0.02). A second parameter analyzed was mean swing time (the time interval between each consecutive placement of the same paw), for which a higher number indicates a deficit. While F2-C6 WT rats showed no difference in mean swing time vs. pre-injury baseline (Fig. 4b, one sample t test p > 0.05), F2-C6-D rats exhibited an increase in comparison with both pre-injury baseline (Fig. 4b, one sample t test #p < 0.05) and F2-C6-WT animals (Student’s t test *p = 0.04). These data indicate a slowed step cycle and decrement in recovery compared to F2-C6 WT. A third parameter analyzed was duty cycle (the percentage of time spent standing within a step cycle), which is indicative of weight bearing. F2-C6-WT rats did not exhibit a significant decrease from pre-injury baseline for duty cycle, but F2-C6-D rats again demonstrated a significant decrement in comparison with both pre-injury baseline (Fig. 4c, one sample t test #p < 0.05), and F2-C6 WT rats (Fig. 4c, Student’s t test *p = 0.03). The fourth parameter analyzed was regularity index (a measure of coordination). Both F2-C6-WT and F2-C6-D rats were significantly impaired vs. pre-injury baseline levels for regularity index (Fig. 4d, one sample t test #p < 0.05); while not reaching significance, a strong trend for a further decrease in F2-C6-D rat was observed in comparison with F2-C6 WT rats (Fig. 4d, Student’s t test p = 0.08).
C6 deficiency alters white matter sparing and lesion volume in homozygous strain H-C6 PVG but not in littermate control F2-C6 PVG rats
We assessed whether C6 deficiency affected percent white matter sparing (Fig. 5a) or lesion volume (Fig. 5b) within the homozygous colony and littermate control cohorts using unbiased stereology. As noted above, statistical comparisons between cohorts should be approached with caution, because these cohorts were run at different times; however, no statistical differences were observed between H-WT and F2-WT rats for either SCI-induced lesion volume (H-WT mean 2.360 ± 0.3300 SEM N = 8), F2-WT 2.873 ± 0.2020 SEM N = 8; p = 0.2061; 2-tailed t test) or percent spared white matter (H-WT mean 23.20 ± 0.980 SEM, F2 WT mean 18.38 ± 2.17 SEM; p = 0.0625; 2-tailed t test). H-C6-D rats showed an increase in percent spared white matter area at the injury epicenter vs. H-C6-WT rats (Fig. 5c). In contrast, this measurement was unchanged between F2-C6-D and F2-C6 WT rats (Fig. 5d, Student’s t test, p = 0.4). Parallel analysis of central lesion volume in the homozygous strain cohort found no difference between H-C6-D vs. H-C6-WT rats (Fig. 5e). However, again in contrast, animals in the littermate control cohort exhibited a strong trend towards increased lesion size in F2-C6-D vs. F2-C6-WT rats (Fig. 5f, Student’s t test, p = 0.08). Taken together these histological data demonstrate divergent responses in lesion pathogenesis as well as locomotor recovery between homozygous colony and littermate control cohorts.
Discussion
Here, we have compared the recovery differences of rats that were either maintained as separate homozygous colonies or generated from F2 crosses to yield littermate controls. Within cohort comparisons demonstrate that H-C6-WT vs. H-C6-D rats and F2-C6-WT vs. F2-C6-D rats have different results for both recovery of function and lesion pathogenesis after SCI. These results highlight the importance of the use of littermate controls in studies involving genetic manipulation of the complement cascade. While future studies should include comparisons between the different cohorts within the same experiment to also test for baseline differences, the current data indicate that there are functional differences due to maintenance in separate homozygous colonies versus heterozygous colonies to generate littermate controls.
The standard protocol in the literature has been to utilize animals from separate homozygous colonies for comparisons of C6 deficiency. A literature search identifying papers utilizing C6 WT and C6-D rats as a component of the experimental work identified 18 studies, a majority of which reported obtaining WT and C6 deficient rats from separate sources, highlighting a need to review findings using this model. Because of identified differences in complement sufficiency and activation between species, the C6-D PVG rat has been an important model for the study of complement and inflammation. C57Bl/6 mice, the most common background for genetically manipulated mice, have dramatically reduced C5b-9-hemolytic capacity in comparison with rats57,58. Indeed, we have previously reported that male C57Bl/6 mice fail to exhibit hemolytic activity in CH50 assays after SCI in comparison with male BUB mice or Sprague Dawley rats58. Accordingly, while transgenic mice can give insight into innate immune mechanisms in inflammation and injury, mouse models may have gaps with regard to the initiation of downstream immune activation. Together, these points highlight the importance of conducting studies in a rat model in which bred-in genetic variation between control and knockout/deletion animals is addressed.
C6-D PVG rats have been previously characterized and reported to derive from a specific autosomal recessive spontaneous mutation59,60; in parallel, tissue antigens, serum levels of other complement proteins, and spleen cell proliferation of C6-D rats have been reported to be identical to that of WT rats sharing the PVG background. Finally, these animals also do not exhibit either evidence of increased vulnerability to infection within a controlled vivarium environment, or evidence of differences at the level of immunity based on mixed lymphocyte reaction and alloantibody testing. However, it should be noted that the data presented cannot exclude the possibility of potential variabilities in blood or other immune parameters at baseline between colonies. Additionally, strain differences in SCI lesion pathogenesis are well recognized61–67. It would thus not be surprising that non-littermate WT and C6-D rats maintained in separate homozygous colonies for generations have diverged, resulting in different functional strain characteristics. In addition to genetic drift with colony maintenance practices, there are a number of reasons why maintenance of animals in separate colonies could yield such a result. For example, obtaining animals from different sources or housing in separate locations may lead to differences within the gut microbiome. Villarino et al. observed that C57Bl/6 mice that were sourced from different vendors, when exposed to the malaria parasite, differed in their severity response68. Gut microbiota has also been implicated in response to experimental autoimmune encephalomyelitis69, SCI70,71, and other CNS injury such as TBI72. In these studies, however, rats for both C6 WT and C6-D were bred in the same vivarium and fed the same chow; accordingly, the more likely scenario is that the differences in behavior and histology between the homozygous C6 WT and C6-D rat colony and heterozygous rat colony are due to the accumulation of genetic differences.
The results reported here suggest a surprising positive role for C5b-9 after nervous system injury, and are in contrast to studies have evaluated complement deficiency or knockout in SCI mice that are not complement sufficient or not bred to establish littermate controls. A positive role for C5b-9 in recovery after SCI could be consistent with the established role of complement in debris clearance, which is critical for regeneration and plasticity in the CNS. Studies have suggested C5b-9 presence can amplify the complement cascade through a positive feedback loop with C1q10,19. Amplification increases the recruitment of macrophages by an increase in C3a and C5a, which would be predicted to promote clearance of myelin debris that could otherwise inhibit remyelination. The presence of myelin and other debris may also indirectly increase stress or toxicity to, or impair the function of, surviving cells, leading to increased cell death as well as delayed remyelination73–78, negatively impacting motor recovery.
In sum, these results suggest that maintenance of separate homozygous colonies is inadequate for testing the effect of C6 deficiency on locomotor and histological recovery after SCI, and that comparison of F2-WT and F2-C6-D PVG rats provides a more appropriate model for assessing the role of complement in CNS injury. Moreover, these data point to a previously unidentified finding, that C5b-9 formation can exert beneficial functions after SCI, and presumably other types on CNS injury and damage.
Materials and methods
Animal numbers and exclusion criteria
For experiments comparing PVG rats maintained as separate homozygous colonies, PVG wildtype rats were purchased from Harlan (Indianapolis, Indiana) and C6 Deficient (C6-D) rats on a Piebald-Viral Glaxo (PVG) background were generously provided by Paul Morgan (University of Wales College of Medicine, U.K.). These strains are abbreviated as homozygous wildtype (H-WT) or homozygous C6-D-PVG), respectively. From these homozygous litters, H-C6 WT (n = 14) and H-C6-D (n = 12) females were used to assess motor function after spinal cord injury. For experiments comparing PVG rats generated as littermate controls, PVG rats WT purchased from Harlan were crossed with the homozygous PVG C6-D rats from the University of Wales, to generate F1 heterozygote C6-D rats at the University of California, Irvine; heterozygous males and females were then crossed to produce F2 litters with wildtype (F2-WT), heterozygous, and C6-D PVG rats (F2-C6-D PVG). F2-WT (n = 11) and F2-C6-D (n = 10) females were used to assess motor function after spinal cord injury. Only females were used in this study to facilitate manual bladder expression after SCI.
3 (WT, n = 2 and C6-D, n = 1) animals were excluded from final analysis; all exclusions were based on Grubbs test identification of outliers in behavioral data and/or post-injury weight monitoring.
Genotyping
WT and C6-D genotypes were determined using PCR of DNA samples extracted from tail clips (Qiagen DNeasy Tissue Kit) followed by restriction enzyme digest and agarose gel electrophoresis. PCR was conducted using Taq PCR Master Mix (Qiagen) for 38 cycles: 4 m 94 °C; 45 s 94 °C; 1 m 50 °C; 1 m 72 °C; 10 m 72 °C. Primer sequences were as follows: C6 forward: TGCAGTAGGAATGGGGCTAA; C6 reverse: GAGAAAAGAGGCATTCCCAGT. PCR products were purified (Qiagen QIAquick PCR purification kit, DNA eluted in 30 µL NEB buffer, and 15 µl of eluted DNA product digested with 1 µl Ava I (New England Biolabs) overnight at 37 °C. PCR product digests were loaded onto a 1.5% agarose gel for electrophoresis and genotype identification relative to 100 bp DNA ladder as shown in Fig. 1a.
Injury model
All experiments were conducted in accordance in an AALAC accredited vivarium with the UCI Institutional Animal Care and Use Committee (IACUC) approval. Rats were anesthetized with isofluorane gas anesthesia. A laminectomy was performed at thoracic vertebrae 9 (T9) and given 200 kilo dyne (kd) contusion injuries at T9 using the Infinite Horizon Impactor (Precision Systems and Instrumentation, Lexington, KY). After the contusion injury, a small piece of gel-foam was placed over the laminectomy location and the muscles overlying the injury was sutured and skin was closed using metal wound clips. Post-operative care included twice daily manual bladder expression until animals regained voluntary micturition, as well as administration of antibiotics and buprenorphine, as described previously79.
Behavioral assessments
All behavioral testing and scoring was performed by individuals blinded to the experimental group and genotype.
Open field locomotion
The Basso Beattie Bresnahan (BBB) scale was utilized to evaluate gross locomotor recovery in injured animals weekly starting from 7 days post-injury (dpi) up to 42 dpi80. The BBB scale goes from 0 to 21 with the higher the BBB score the more functional the animal.
Horizontal ladderbeam
The horizontal ladder beam task was used as a terminal supplemental quantitative task with higher the number of errors, the less functional the animal56,81–85. Animals were tested at the end of the study prior to sacrifice. Prior to testing and video acquisition, rats were trained in a 20–30 m acclimation session. The apparatus length was 94.5 cm with 20 rungs spaced 2.54 cm apart. During the testing session, rats were videotaped from below; quantification of hindlimb errors was scored by slow motion video playback. Hindlimb errors from three test trials per rat were averaged for subsequent statistical analysis.
CatWalk gait assessment
Catwalk XT (version 7.1 Noldus Information Technology) was used to assess fine details of gait changes and allowed for easy quantification of a large number of gait parameters while animals are recorded crossing a walkway. Prior to testing and video acquisition, rats were trained in an acclimation session. Animals were recorded crossing the catwalk in the dark and data from three test trial per rat were averaged for statistical analysis.
Tissue collection, sectioning and immunohistochemistry
At time of sacrifice, animals were perfused with 4% phosphate-buffered saline (PBS), followed by 4% paraformaldehyde in PBS. The T6–T12 segment of the spinal cord was dissected by the dorsal root to provide an anatomically defined region for stereology. Cords were further post-fixed in 20% sucrose/4% paraformaldehyde in PBS overnight at 4 °C. Spinal cords were frozen in isopentane at − 65 °C and stored at − 80 °C. Serial 30 μm thick coronal cryostat sections were cut on a CryoJane tape-transfer system (Leica Microsystems Inc., Cuffalo Grove, IL) at − 21 °C and collected in sets of 12 for immunohistochemistry.
White matter sparing and lesion volume
Slides were processed for antigen retrieval using a Buffer A (pH 6) in the Retriever 2100 system (PickCell Laboratories, Amsterdam, The Netherlands) before immunohistochemical staining. To assess white matter sparing, slides (1/12 section sampling) were dehydrated through a series of ethanol solutions (50%, 1 min; 70%, 3 min; 95%, 3 min; 100%, 5 min) and then rehydrated back through the alcohol series with fresh ethanol starting at 100% to 50% prior to incubation with anti-myelin basic protein primary antibody overnight (EMD Millipore). Anti-MBP was used at 1:750 and visualized with diaminobenzidine (DAB, Vector Labs, Carpinteria, CA). To assess central lesion volume, slides (1/12 section sampling) were incubated with anti-GFAP overnight (Dako). Anti-GFAP was used at 1:10,000 and visualized with diaminobenzidine (DAB, Vector Labs, Carpinteria, CA).
C5b-9 formation
Slides were processed for antigen retrieval using a trypsin buffer before immunohistochemical staining. To assess C5b-9 formation, mouse monoclonal antibody to Human SC5b-9 (Quidel A239) was used at 1:100 and was visualized with Donkey anti-mouse Alexa-flour 488 Fab (Jackson Immunoresearch) at a 1:500 dilution. A Hoescht counter stain at a dilution of 1:1000 was used to visual nuclei. Images were taken in the ventral horn using the Keyence BZ-X810 and a 60 × objective.
Stereology
Stereological analyses for MBP and GFAP volume were performed on coronal sections (40–44 sections per animal) at 1/12 section sampling (360 µm apart) using StereoInvestigator software (Microbrightfield, Inc) using a 20 × objective. The Cavalieri estimator was used to quantify lesion volume, spared white matter volume, and percent spared white matter area. Quantification was performed by placing a random counting grid (100 μm × 100 μm) and markers that fell within the region of interest were counted. This data was used in the analysis to determined empirically a coefficient of error value that was < 0.10 for examined tissues. All histological analyses were performed by individuals blinded to group and genotype.
Statistics
Prior to statistical analysis was performed a Grubbs’ test was performed to identify potential outliers from both behavioral and histological groups (α = 0.05), removing no more than a single outlier (non-iterative). Comparisons between C6 WT and C6-D rats for BBB were performed using repeated measures 2-way ANOVA with Sidak post-hoc test (Prism; GraphPad, San Diego, CA, USA). Catwalk data was normalized to each individual animal’s pre-injury value and comparisons performed using one sample t test analysis. Histological volume comparisons were conducted by Student’s t test, and MBP distribution from the lesion epicenter was conducted using repeated measures 2-way ANOVA.
Supplementary information
Acknowledgements
This work was supported by funding from the National Institute of Neurological Disorders and Stroke RO1 NS43428-01. We also thank Hongli Liu for her assistance with animal surgeries and behavioral assessments and our undergraduate Samar Bhat for his assistance with quantification.
Author contributions
Conceived and designed the experiments: M.D.G., B.J.C., and A.J.A. Performed the experiments: D.S. and M.D.G. Analyzed the data: D.S., M.J.H., R.A.N. and M.D.G. Prepared the manuscript: D.S., M.J.H., and A.J.A. All authors have read and approved the final manuscript.
Competing interests
The authors declare no competing interests.
Footnotes
Publisher's note
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
These authors contributed equally: Diane Su and Mitra J. Hooshmand.
Supplementary information
is available for this paper at 10.1038/s41598-020-76441-3.
References
- 1.Beck KD, et al. Quantitative analysis of cellular inflammation after traumatic spinal cord injury: Evidence for a multiphasic inflammatory response in the acute to chronic environment. Brain j. Neurol. 2010;133:433–447. doi: 10.1093/brain/awp322. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 2.Oyinbo CA. Secondary injury mechanisms in traumatic spinal cord injury: A nugget of this multiply cascade. Acta Neurobiol. Exp. (Wars) 2011;71:281–299. doi: 10.55782/ane-2011-1848. [DOI] [PubMed] [Google Scholar]
- 3.Zhang N, Yin Y, Xu SJ, Wu YP, Chen WS. Inflammation and apoptosis in spinal cord injury. Indian J. Med. Res. 2012;135:287–296. [PMC free article] [PubMed] [Google Scholar]
- 4.Peterson SL, Nguyen HX, Mendez OA, Anderson AJ. Complement protein C3 suppresses axon growth and promotes neuron loss. Sci. Rep. 2017;7:12904. doi: 10.1038/s41598-017-11410-x. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 5.Haefliger JA, Tschopp J, Vial N, Jenne DE. Complete primary structure and functional characterization of the sixth component of the human complement system. Identification of the C5b-binding domain in complement C6. J. Biol. Chem. 1989;264:18041–18051. [PubMed] [Google Scholar]
- 6.Tegla CA, et al. Membrane attack by complement: The assembly and biology of terminal complement complexes. Immunol. Res. 2011;51:45–60. doi: 10.1007/s12026-011-8239-5. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 7.Nataf S, Carroll SL, Wetsel RA, Szalai AJ, Barnum SR. Attenuation of experimental autoimmune demyelination in complement-deficient mice. J. Immunol. 2000;165:5867–5873. doi: 10.4049/jimmunol.165.10.5867. [DOI] [PubMed] [Google Scholar]
- 8.Mead RJ, Singhrao SK, Neal JW, Lassmann H, Morgan BP. The membrane attack complex of complement causes severe demyelination associated with acute axonal injury. J. Immunol. 2002;168:458–465. doi: 10.4049/jimmunol.168.1.458. [DOI] [PubMed] [Google Scholar]
- 9.Qiao F, et al. Complement plays an important role in spinal cord injury and represents a therapeutic target for improving recovery following trauma. Am. J. Pathol. 2006;169:1039–1047. doi: 10.2353/ajpath.2006.060248. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 10.Ramaglia V, et al. The membrane attack complex of the complement system is essential for rapid Wallerian degeneration. J. Nneurosci. 2007;27:7663–7672. doi: 10.1523/JNEUROSCI.5623-06.2007. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 11.Qiao F, et al. The alternative and terminal pathways of complement mediate post-traumatic spinal cord inflammation and injury. Am. J. Pathol. 2010;177:3061–3070. doi: 10.2353/ajpath.2010.100158. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 12.Stahel PF, Flierl MA. Targeted modulation of the neuroinflammatory response after spinal cord injury: The ongoing quest for the "holy grail". Am. J. Pathol. 2010;177:2685–2687. doi: 10.2353/ajpath.2010.100408. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 13.Scolding NJ, et al. Normal rat serum cytotoxicity against syngeneic oligodendrocytes. Complement activation and attack in the absence of anti-myelin antibodies. J. Neurol. Sci. 1989;89:289–300. doi: 10.1016/0022-510X(89)90030-0. [DOI] [PubMed] [Google Scholar]
- 14.Wren DR, Noble M. Oligodendrocytes and oligodendrocyte/type-2 astrocyte progenitor cells of adult rats are specifically susceptible to the lytic effects of complement in absence of antibody. Proc. Natl. Acad. Sci. USA. 1989;86:9025–9029. doi: 10.1073/pnas.86.22.9025. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 15.Piddlesden SJ, Morgan BP. Killing of rat glial cells by complement: Deficiency of the rat analogue of CD59 is the cause of oligodendrocyte susceptibility to lysis. J. Neuroimmunol. 1993;48:169–175. doi: 10.1016/0165-5728(93)90189-6. [DOI] [PubMed] [Google Scholar]
- 16.Agoropoulou C, Piddlesden SJ, Lachmann PJ, Wing MG. Neuronal protection of oligodendrocytes from antibody-independent complement lysis. NeuroReport. 1998;9:927–932. doi: 10.1097/00001756-199803300-00030. [DOI] [PubMed] [Google Scholar]
- 17.Singhrao SK, Neal JW, Rushmere NK, Morgan BP, Gasque P. Spontaneous classical pathway activation and deficiency of membrane regulators render human neurons susceptible to complement lysis. Am. J. Pathol. 2000;157:905–918. doi: 10.1016/S0002-9440(10)64604-4. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 18.Yao X, Verkman AS. Marked central nervous system pathology in CD59 knockout rats following passive transfer of Neuromyelitis optica immunoglobulin G. Acta Neuropathol. Commun. 2017;5:15. doi: 10.1186/s40478-017-0417-9. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 19.Tran GT, et al. Attenuation of experimental allergic encephalomyelitis in complement component 6-deficient rats is associated with reduced complement C9 deposition, P-selectin expression, and cellular infiltrate in spinal cords. J. Immunol. 2002;168:4293–4300. doi: 10.4049/jimmunol.168.9.4293. [DOI] [PubMed] [Google Scholar]
- 20.Castellano G, et al. Pentraxin 3 and complement cascade activation in the failure of arteriovenous fistula. Atherosclerosis. 2010;209:241–247. doi: 10.1016/j.atherosclerosis.2009.08.044. [DOI] [PubMed] [Google Scholar]
- 21.Lewis RD, Jackson CL, Morgan BP, Hughes TR. The membrane attack complex of complement drives the progression of atherosclerosis in apolipoprotein E knockout mice. Mol. Immunol. 2010;47:1098–1105. doi: 10.1016/j.molimm.2009.10.035. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 22.ter Weeme M, et al. Activated complement is more extensively present in diseased aortic valves than naturally occurring complement inhibitors: A sign of ongoing inflammation. Eur. J. Clin. Invest. 2010;40:4–10. doi: 10.1111/j.1365-2362.2009.02216.x. [DOI] [PubMed] [Google Scholar]
- 23.Knoess M, et al. Colocalization of C4d deposits/CD68+ macrophages in rheumatoid nodule and granuloma annulare: Immunohistochemical evidence of a complement-mediated mechanism in fibrinoid necrosis. Pathol. Res. Pract. 2008;204:373–378. doi: 10.1016/j.prp.2008.01.009. [DOI] [PubMed] [Google Scholar]
- 24.Corallini F, et al. The soluble terminal complement complex (SC5b-9) up-regulates osteoprotegerin expression and release by endothelial cells: Implications in rheumatoid arthritis. Rheumatology (Oxford) 2009;48:293–298. doi: 10.1093/rheumatology/ken495. [DOI] [PubMed] [Google Scholar]
- 25.Alexander JJ, Anderson AJ, Barnum SR, Stevens B, Tenner AJ. The complement cascade: Yin-Yang in neuroinflammation–neuro-protection and -degeneration. J. Neurochem. 2008;107:1169–1187. doi: 10.1111/j.1471-4159.2008.05668.x. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 26.Kolev MV, Ruseva MM, Harris CL, Morgan BP, Donev RM. Implication of complement system and its regulators in Alzheimer's disease. Curr. Neuropharmacol. 2009;7:1–8. doi: 10.2174/157015909787602805. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 27.Singhrao SK, Neal JW, Morgan BP, Gasque P. Increased complement biosynthesis by microglia and complement activation on neurons in Huntington's disease. Exp. Neurol. 1999;159:362–376. doi: 10.1006/exnr.1999.7170. [DOI] [PubMed] [Google Scholar]
- 28.Yasuhara O, et al. Pick's disease immunohistochemistry: New alterations and Alzheimer's disease comparisons. Acta Neuropathol. 1995;89:322–330. doi: 10.1007/BF00309625. [DOI] [PubMed] [Google Scholar]
- 29.Morgan BP. Complement membrane attack on nucleated cells: Resistance, recovery and non-lethal effects. Biochem. J. 1989;264:1–14. doi: 10.1042/bj2640001. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 30.Kilgore KS, et al. Sublytic concentrations of the membrane attack complex of complement induce endothelial interleukin-8 and monocyte chemoattractant protein-1 through nuclear factor-kappa B activation. Am. J. Pathol. 1997;150:2019–2031. [PMC free article] [PubMed] [Google Scholar]
- 31.Dashiell SM, Rus H, Koski CL. Terminal complement complexes concomitantly stimulate proliferation and rescue of Schwann cells from apoptosis. Glia. 2000;30:187–198. doi: 10.1002/(SICI)1098-1136(200004)30:2<187::AID-GLIA8>3.0.CO;2-7. [DOI] [PubMed] [Google Scholar]
- 32.Hila S, Soane L, Koski CL. Sublytic C5b-9-stimulated Schwann cell survival through PI 3-kinase-mediated phosphorylation of BAD. Glia. 2001;36:58–67. doi: 10.1002/glia.1095. [DOI] [PubMed] [Google Scholar]
- 33.Rus HG, Niculescu FI, Shin ML. Role of the C5b–9 complement complex in cell cycle and apoptosis. Immunol. Rev. 2001;180:49–55. doi: 10.1034/j.1600-065X.2001.1800104.x. [DOI] [PubMed] [Google Scholar]
- 34.Soane L, Cho HJ, Niculescu F, Rus H, Shin ML. C5b–9 terminal complement complex protects oligodendrocytes from death by regulating Bad through phosphatidylinositol 3-kinase/Akt pathway. J. Immunol. 2001;167:2305–2311. doi: 10.4049/jimmunol.167.4.2305. [DOI] [PubMed] [Google Scholar]
- 35.Fosbrink M, Niculescu F, Rus H. The role of c5b–9 terminal complement complex in activation of the cell cycle and transcription. Immunol. Res. 2005;31:37–46. doi: 10.1385/IR:31:1:37. [DOI] [PubMed] [Google Scholar]
- 36.Cudrici C, Niculescu T, Niculescu F, Shin ML, Rus H. Oligodendrocyte cell death in pathogenesis of multiple sclerosis: Protection of oligodendrocytes from apoptosis by complement. J. Rehabil. Res. Dev. 2006;43:123–132. doi: 10.1682/JRRD.2004.08.0111. [DOI] [PubMed] [Google Scholar]
- 37.Tegla CA, et al. Neuroprotective effects of the complement terminal pathway during demyelination: Implications for oligodendrocyte survival. J. Neuroimmunol. 2009;213:3–11. doi: 10.1016/j.jneuroim.2009.06.006. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 38.Toropainen M, Saarinen L, Vidarsson G, Kayhty H. Protection by meningococcal outer membrane protein PorA-specific antibodies and a serogroup B capsular polysaccharide-specific antibody in complement-sufficient and C6-deficient infant rats. Infect. Immun. 2006;74:2803–2808. doi: 10.1128/IAI.74.5.2803-2808.2006. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 39.Tran GT, et al. Membrane attack complex of complement is not essential for immune mediated demyelination in experimental autoimmune neuritis. J. Neuroimmunol. 2010;229:98–106. doi: 10.1016/j.jneuroim.2010.07.010. [DOI] [PubMed] [Google Scholar]
- 40.Brauer RB, et al. Endotoxin-induced lung inflammation is independent of the complement membrane attack complex. Infect. Immun. 2000;68:1626–1632. doi: 10.1128/iai.68.3.1626-1632.2000. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 41.Fischetti F, et al. Selective therapeutic control of C5a and the terminal complement complex by anti-C5 single-chain Fv in an experimental model of antigen-induced arthritis in rats. Arthritis Rheum. 2007;56:1187–1197. doi: 10.1002/art.22492. [DOI] [PubMed] [Google Scholar]
- 42.Fischetti F, et al. Innate immunity, through late complement components activation, contributes to the development of early vascular inflammation and morphologic alterations in experimental diabetes. Atherosclerosis. 2011;216:83–89. doi: 10.1016/j.atherosclerosis.2011.01.050. [DOI] [PubMed] [Google Scholar]
- 43.Holtman L, van Vliet EA, Baas F, Aronica E, Gorter JA. Complement protein 6 deficiency in PVG/c rats does not lead to neuroprotection against seizure induced cell death. Neuroscience. 2011;188:109–116. doi: 10.1016/j.neuroscience.2011.05.003. [DOI] [PubMed] [Google Scholar]
- 44.Rangan GK, Pippin JW, Couser WG. C5b–9 regulates peritubular myofibroblast accumulation in experimental focal segmental glomerulosclerosis. Kidney Int. 2004;66:1838–1848. doi: 10.1111/j.1523-1755.2004.00957.x. [DOI] [PubMed] [Google Scholar]
- 45.Nangaku M, Pippin J, Couser WG. C6 mediates chronic progression of tubulointerstitial damage in rats with remnant kidneys. J. Am. Soc. Nephrol. 2002;13:928–936. doi: 10.1681/ASN.V134928. [DOI] [PubMed] [Google Scholar]
- 46.Rangan GK, Pippin JW, Coombes JD, Couser WG. C5b–9 does not mediate chronic tubulointerstitial disease in the absence of proteinuria. Kidney Int. 2005;67:492–503. doi: 10.1111/j.1523-1755.2005.67106.x. [DOI] [PubMed] [Google Scholar]
- 47.Nangaku M, et al. Renal microvascular injury induced by antibody to glomerular endothelial cells is mediated by C5b–9. Kidney Int. 1997;52:1570–1578. doi: 10.1038/ki.1997.487. [DOI] [PubMed] [Google Scholar]
- 48.Nangaku M, Pippin J, Couser WG. Complement membrane attack complex (C5b–9) mediates interstitial disease in experimental nephrotic syndrome. J. Am. Soc. Nephrol. 1999;10:2323–2331. doi: 10.1681/ASN.V10112323. [DOI] [PubMed] [Google Scholar]
- 49.Spicer ST, et al. Induction of passive Heymann nephritis in complement component 6-deficient PVG rats. J. Immunol. 2007;179:172–178. doi: 10.4049/jimmunol.179.1.172. [DOI] [PubMed] [Google Scholar]
- 50.Leenaerts PL, Hall BM, Van Damme BJ, Daha MR, Vanrenterghem YF. Active Heymann nephritis in complement component C6 deficient rats. Kidney Int. 1995;47:1604–1614. doi: 10.1038/ki.1995.224. [DOI] [PubMed] [Google Scholar]
- 51.Sato T, et al. The terminal sequence of complement plays an essential role in antibody-mediated renal cell apoptosis. J. Am. Soc. Nephrol. 1999;10:1242–1252. doi: 10.1681/ASN.V1061242. [DOI] [PubMed] [Google Scholar]
- 52.Brandt J, et al. Role of the complement membrane attack complex (C5b–9) in mediating experimental mesangioproliferative glomerulonephritis. Kidney Int. 1996;49:335–343. doi: 10.1038/ki.1996.50. [DOI] [PubMed] [Google Scholar]
- 53.Hughes J, et al. C5b–9 membrane attack complex mediates endothelial cell apoptosis in experimental glomerulonephritis. Am. J. Physiol. Renal. Physiol. 2000;278:F747–757. doi: 10.1152/ajprenal.2000.278.5.F747. [DOI] [PubMed] [Google Scholar]
- 54.Anderson AJ, Robert S, Huang W, Young W, Cotman CW. Activation of complement pathways after contusion-induced spinal cord injury. J. Neurotrauma. 2004;21:1831–1846. doi: 10.1089/neu.2004.21.1831. [DOI] [PubMed] [Google Scholar]
- 55.Anderson AJ, Najbauer J, Huang W, Young W, Robert S. Upregulation of complement inhibitors in association with vulnerable cells following contusion-induced spinal cord injury. J. Neurotrauma. 2005;22:382–397. doi: 10.1089/neu.2005.22.382. [DOI] [PubMed] [Google Scholar]
- 56.Cummings BJ, Engesser-Cesar C, Cadena G, Anderson AJ. Adaptation of a ladder beam walking task to assess locomotor recovery in mice following spinal cord injury. Behav. Brain Res. 2007;177:232–241. doi: 10.1016/j.bbr.2006.11.042. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 57.Ong GL, Mattes MJ. Mouse strains with typical mammalian levels of complement activity. J. Immunol. Methods. 1989;125:147–158. doi: 10.1016/0022-1759(89)90088-4. [DOI] [PubMed] [Google Scholar]
- 58.Galvan MD, et al. Deficiency in complement C1q improves histological and functional locomotor outcome after spinal cord injury. J. Nneurosci. 2008;28:13876–13888. doi: 10.1523/JNEUROSCI.2823-08.2008. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 59.van Dixhoorn MG, et al. Characterization of complement C6 deficiency in a PVG/c rat strain. Clin. Exp. Immunol. 1997;109:387–396. doi: 10.1046/j.1365-2249.1997.4551354.x. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 60.Leenaerts PL, et al. Hereditary C6 deficiency in a strain of PVG/c rats. Clin. Exp. Immunol. 1994;97:478–482. doi: 10.1111/j.1365-2249.1994.tb06113.x. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 61.Basso DM, et al. Basso Mouse Scale for locomotion detects differences in recovery after spinal cord injury in five common mouse strains. J. Neurotrauma. 2006;23:635–659. doi: 10.1089/neu.2006.23.635. [DOI] [PubMed] [Google Scholar]
- 62.Kigerl KA, McGaughy VM, Popovich PG. Comparative analysis of lesion development and intraspinal inflammation in four strains of mice following spinal contusion injury. J. Comp. Neurol. 2006;494:578–594. doi: 10.1002/cne.20827. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 63.Kostyk SK, Popovich PG, Stokes BT, Wei P, Jakeman LB. Robust axonal growth and a blunted macrophage response are associated with impaired functional recovery after spinal cord injury in the MRL/MpJ mouse. Neuroscience. 2008;156:498–514. doi: 10.1016/j.neuroscience.2008.08.013. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 64.Noristani HN, They L, Perrin FE. C57BL/6 and Swiss Webster Mice display differences in mobility, gliosis, microcavity formation and lesion volume after severe spinal cord injury. Front. Cell Neurosci. 2018;12:173. doi: 10.3389/fncel.2018.00173. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 65.Noristani HN, et al. Longitudinal magnetic resonance imaging analysis and histological characterization after spinal cord injury in two mouse strains with different functional recovery: Gliosis as a key factor. J. Neurotrauma. 2018;35:2924–2940. doi: 10.1089/neu.2017.5613. [DOI] [PubMed] [Google Scholar]
- 66.Popovich PG, Wei P, Stokes BT. Cellular inflammatory response after spinal cord injury in Sprague–Dawley and Lewis rats. J. Comp. Neurol. 1997;377:443–464. doi: 10.1002/(SICI)1096-9861(19970120)377:3<443::AID-CNE10>3.0.CO;2-S. [DOI] [PubMed] [Google Scholar]
- 67.Inman D, Guth L, Steward O. Genetic influences on secondary degeneration and wound healing following spinal cord injury in various strains of mice. J. Comp. Neurol. 2002;451:225–235. doi: 10.1002/cne.10340. [DOI] [PubMed] [Google Scholar]
- 68.Villarino NF, et al. Composition of the gut microbiota modulates the severity of malaria. Proc. Natl. Acad. Sci. USA. 2016;113:2235–2240. doi: 10.1073/pnas.1504887113. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 69.Ochoa-Reparaz J, et al. Role of gut commensal microflora in the development of experimental autoimmune encephalomyelitis. J. Immunol. 2009;183:6041–6050. doi: 10.4049/jimmunol.0900747. [DOI] [PubMed] [Google Scholar]
- 70.Kigerl KA, Mostacada K, Popovich PG. Gut microbiota are disease-modifying factors after traumatic spinal cord injury. Neurotherapeutics. 2018;15:60–67. doi: 10.1007/s13311-017-0583-2. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 71.Kigerl KA, et al. Gut dysbiosis impairs recovery after spinal cord injury. J. Exp. Med. 2016;213:2603–2620. doi: 10.1084/jem.20151345. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 72.Sundman MH, Chen NK, Subbian V, Chou YH. The bidirectional gut-brain-microbiota axis as a potential nexus between traumatic brain injury, inflammation, and disease. Brain Behav. Immunol. 2017;66:31–44. doi: 10.1016/j.bbi.2017.05.009. [DOI] [PubMed] [Google Scholar]
- 73.Graca DL, Blakemore WF. Delayed remyelination in rat spinal cord following ethidium bromide injection. Neuropathol. Appl. Neurobiol. 1986;12:593–605. doi: 10.1111/j.1365-2990.1986.tb00162.x. [DOI] [PubMed] [Google Scholar]
- 74.McKerracher L, et al. Identification of myelin-associated glycoprotein as a major myelin-derived inhibitor of neurite growth. Neuron. 1994;13:805–811. doi: 10.1016/0896-6273(94)90247-X. [DOI] [PubMed] [Google Scholar]
- 75.Mukhopadhyay G, Doherty P, Walsh FS, Crocker PR, Filbin MT. A novel role for myelin-associated glycoprotein as an inhibitor of axonal regeneration. Neuron. 1994;13:757–767. doi: 10.1016/0896-6273(94)90042-6. [DOI] [PubMed] [Google Scholar]
- 76.Shields S, Gilson J, Blakemore W, Franklin R. Remyelination occurs as extensively but more slowly in old rats compared to young rats following fliotoxin-induced CNS demyelination. Glia. 2000;29:102. doi: 10.1002/(SICI)1098-1136(20000101)29:1<102::AID-GLIA12>3.0.CO;2-1. [DOI] [PubMed] [Google Scholar]
- 77.Ibanez C, et al. Systemic progesterone administration results in a partial reversal of the age-associated decline in CNS remyelination following toxin-induced demyelination in male rats. Neuropathol. Appl. Neurobiol. 2004;30:80–89. doi: 10.1046/j.0305-1846.2003.00515.x. [DOI] [PubMed] [Google Scholar]
- 78.Rotshenker S. Wallerian degeneration: The innate-immune response to traumatic nerve injury. J. Neuroinflamm. 2011;8:109. doi: 10.1186/1742-2094-8-109. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 79.Nguyen HX, Galvan MD, Anderson AJ. Characterization of early and terminal complement proteins associated with polymorphonuclear leukocytes in vitro and in vivo after spinal cord injury. J. Neuroinflamm. 2008;5:26. doi: 10.1186/1742-2094-5-26. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 80.Basso DM, Beattie MS, Bresnahan JC. A sensitive and reliable locomotor rating scale for open field testing in rats. J. Neurotrauma. 1995;12:1–21. doi: 10.1089/neu.1995.12.1. [DOI] [PubMed] [Google Scholar]
- 81.Bolton DA, Tse AD, Ballermann M, Misiaszek JE, Fouad K. Task specific adaptations in rat locomotion: Runway versus horizontal ladder. Behav. Brain Res. 2006;168:272–279. doi: 10.1016/j.bbr.2005.11.017. [DOI] [PubMed] [Google Scholar]
- 82.Gensel JC, et al. Behavioral and histological characterization of unilateral cervical spinal cord contusion injury in rats. J. Neurotrauma. 2006;23:36–54. doi: 10.1089/neu.2006.23.36. [DOI] [PubMed] [Google Scholar]
- 83.Chan CC, et al. Dose-dependent beneficial and detrimental effects of ROCK inhibitor Y27632 on axonal sprouting and functional recovery after rat spinal cord injury. Exp. Neurol. 2005;196:352–364. doi: 10.1016/j.expneurol.2005.08.011. [DOI] [PubMed] [Google Scholar]
- 84.Liebscher T, et al. Nogo-A antibody improves regeneration and locomotion of spinal cord-injured rats. Ann. Neurol. 2005;58:706–719. doi: 10.1002/ana.20627. [DOI] [PubMed] [Google Scholar]
- 85.Hooshmand, M. J. et al. Complement proteins C1q and C3a promote migration and astroglial differentiation of human neural stem cells (2013b).
Associated Data
This section collects any data citations, data availability statements, or supplementary materials included in this article.