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Nerve regeneration by intravenous administration of human amniotic fluid mesenchymal stem cells regulated by SDF-1α in a sciatic nerve injury model
|關鍵字:||amniotic fluid mesenchymal stem cells;羊水間葉幹細胞;stromal derived factor -1α;chemokine receptor type 4;基質衍生因子-1α;第4型趨化因子接受體||出版社:||生命科學院碩士在職專班||引用:||1 Kandel ER, S. J., Jessell TM. Principle of Neural Science. (McGraw Hill, 2000). 2 A.R.Crossman., D. N. An illustrate color text: NEUROANATOMY. (Churchill Livingstone, 2010). 3 Griffin JW, K. G., Trapp BD. Peripheral neuropathy. (WB Sanders Co., 1993). 4 G, L. Nerve Injury and Repair. (Churchill Livingstone, 1988). 5 H., S. Surgical of Disorders of the Peripheral Nerves. (Williams and Wilkins, 1975). 6 S., S. Nerves and Nerve Injuries. (Churchill Livingstone, 1981). 7 Fawcett JW, K. R. Peripheral nerve regeneration., (Annu Revneurosci, 1990). 8 B., K. Methods of Tissue Engineering. (Gulf Professional 2002). 9 Lin, K.-L. et al. DuraSeal as a Ligature in the Anastomosis of Rat Sciatic Nerve Gap Injury. Journal of Surgical Research 161, 101-110, doi:10.1016/j.jss.2008.10.020 (2010). 10 Pan H.C Fau - Sheu, M.-L. et al. - Magnesium supplement promotes sciatic nerve regeneration and down-regulates inflammatory response. Magnes Res 24, 54-70 (2011). 11 Pan H.C Fau - Cheng, F.-C. et al. - Dietary supplement with fermented soybeans, natto, improved the neurobehavioral deficits after sciatic nerve injury in rats. Neurol Res 31, 441-452 (2009). 12 Murakami, T. et al. Transplanted neuronal progenitor cells in a peripheral nerve gap promote nerve repair. Brain Research 974, 17-24, doi:10.1016/s0006-8993(03)02539-3 (2003). 13 Pan, H.-C. et al. Post-injury regeneration in rat sciatic nerve facilitated by neurotrophic factors secreted by amniotic fluid mesenchymal stem cells. Journal of Clinical Neuroscience 14, 1089-1098, doi:10.1016/j.jocn.2006.08.008 (2007). 14 Pan, H. C. et al. Enhanced regeneration in injured sciatic nerve by human amniotic mesenchymal stem cell. Journal of clinical neuroscience : official journal of the Neurosurgical Society of Australasia 13, 570-575, doi:10.1016/j.jocn.2005.06.007 (2006). 15 M, P. Curr Opin Neurol. (1995). 16 Dezawa, M., Takahashi, I., Esaki, M., Takano, M. & Sawada, H. Sciatic nerve regeneration in rats induced by transplantation of in vitro differentiated bone-marrow stromal cells. The European journal of neuroscience 14, 1771-1776 (2001). 17 Shen, Z. L. et al. Viability of cultured nerve grafts: An assessment of proliferation of Schwann cells and fibroblasts. Microsurgery 19, 356-363 (1999). 18 Inoue, M., Hojo, T., Yano, T. & Katsumi, Y. The effects of electroacupuncture on peripheral nerve regeneration in rats. Acupuncture in medicine : journal of the British Medical Acupuncture Society 21, 9-17 (2003). 19 Vleggeert-Lankamp, C. L. et al. Adhesion and proliferation of human Schwann cells on adhesive coatings. Biomaterials 25, 2741-2751, doi:10.1016/j.biomaterials.2003.09.067 (2004). 20 Buhnemann, C. et al. Neuronal differentiation of transplanted embryonic stem cell-derived precursors in stroke lesions of adult rats. Brain : a journal of neurology 129, 3238-3248, doi:10.1093/brain/awl261 (2006). 21 Su, H. L. et al. Generation of cerebellar neuron precursors from embryonic stem cells. Developmental biology 290, 287-296, doi:10.1016/j.ydbio.2005.11.010 (2006). 22 Pan, H. C. et al. Characterization of axon formation in the embryonic stem cell-derived motoneuron. Cell transplantation 20, 493-502, doi:10.3727/096368910x536464 (2011). 23 Takahashi, K. & Yamanaka, S. Induction of pluripotent stem cells from mouse embryonic and adult fibroblast cultures by defined factors. Cell 126, 663-676, doi:10.1016/j.cell.2006.07.024 (2006). 24 Yu, J. et al. Induced pluripotent stem cell lines derived from human somatic cells. Science (New York, N.Y.) 318, 1917-1920, doi:10.1126/science.1151526 (2007). 25 Vierbuchen, T. et al. Direct conversion of fibroblasts to functional neurons by defined factors. Nature 463, 1035-1041, doi:http://www.nature.com/nature/journal/v463/n7284/suppinfo/nature08797_S1.html (2010). 26 Hussein, S. M. et al. Copy number variation and selection during reprogramming to pluripotency. Nature 471, 58-62 (2011). 27 Gore, A. et al. Somatic coding mutations in human induced pluripotent stem cells. Nature 471, 63-67 (2011). 28 Chen, J. et al. Intravenous administration of human umbilical cord blood reduces behavioral deficits after stroke in rats. Stroke; a journal of cerebral circulation 32, 2682-2688 (2001). 29 Kang, K. S. et al. A 37-year-old spinal cord-injured female patient, transplanted of multipotent stem cells from human UC blood, with improved sensory perception and mobility, both functionally and morphologically: a case study. Cytotherapy 7, 368-373, doi:10.1080/14653240500238160 (2005). 30 Koda M Fau - Nishio, Y. et al. - Granulocyte colony-stimulating factor (G-CSF) mobilizes bone marrow-derived cells into injured spinal cord and promotes functional recovery after compression-induced spinal cord injury in mice. Brain Res 29, 223-231 (2007). 31 Pan, H. C. et al. Potentiation of angiogenesis and regeneration by G-CSF after sciatic nerve crush injury. Biochemical and biophysical research communications 382, 177-182, doi:10.1016/j.bbrc.2009.03.003 (2009). 32 Tsai, M. S. et al. Clonal amniotic fluid-derived stem cells express characteristics of both mesenchymal and neural stem cells. Biology of reproduction 74, 545-551, doi:10.1095/biolreprod.105.046029 (2006). 33 Cheng, F. C. et al. Enhancement of regeneration with glia cell line-derived neurotrophic factor-transduced human amniotic fluid mesenchymal stem cells after sciatic nerve crush injury. Journal of neurosurgery 112, 868-879, doi:10.3171/2009.8.jns09850 (2010). 34 Pan, H. C. et al. Human amniotic fluid mesenchymal stem cells in combination with hyperbaric oxygen augment peripheral nerve regeneration. Neurochemical research 34, 1304-1316, doi:10.1007/s11064-008-9910-7 (2009). 35 Pan, H. C. et al. Combination of G-CSF administration and human amniotic fluid mesenchymal stem cell transplantation promotes peripheral nerve regeneration. Neurochemical research 34, 518-527, doi:10.1007/s11064-008-9815-5 (2009). 36 Nagaya, N. et al. Intravenous administration of mesenchymal stem cells improves cardiac function in rats with acute myocardial infarction through angiogenesis and myogenesis. American journal of physiology. Heart and circulatory physiology 287, H2670-2676, doi:10.1152/ajpheart.01071.2003 (2004). 37 Wang, F. et al. Intravenous administration of mesenchymal stem cells exerts therapeutic effects on parkinsonian model of rats: focusing on neuroprotective effects of stromal cell-derived factor-1alpha. BMC neuroscience 11, 52, doi:10.1186/1471-2202-11-52 (2010). 38 Fischer, U. M. et al. Pulmonary passage is a major obstacle for intravenous stem cell delivery: the pulmonary first-pass effect. Stem cells and development 18, 683-692, doi:10.1089/scd.2008.0253 (2009). 39 Zhang, M. et al. SDF-1 expression by mesenchymal stem cells results in trophic support of cardiac myocytes after myocardial infarction. FASEB journal : official publication of the Federation of American Societies for Experimental Biology 21, 3197-3207, doi:10.1096/fj.06-6558com (2007). 40 Doitsidou, M. et al. Guidance of primordial germ cell migration by the chemokine SDF-1. Cell 111, 647-659 (2002). 41 Molyneaux, K. A. et al. The chemokine SDF1/CXCL12 and its receptor CXCR4 regulate mouse germ cell migration and survival. Development (Cambridge, England) 130, 4279-4286 (2003). 42 Ara, T. et al. Impaired colonization of the gonads by primordial germ cells in mice lacking a chemokine, stromal cell-derived factor-1 (SDF-1). Proceedings of the National Academy of Sciences of the United States of America 100, 5319-5323, doi:10.1073/pnas.0730719100 (2003). 43 Ma, Q. et al. Impaired B-lymphopoiesis, myelopoiesis, and derailed cerebellar neuron migration in CXCR4- and SDF-1-deficient mice. Proceedings of the National Academy of Sciences of the United States of America 95, 9448-9453 (1998). 44 Zheng H Fau - Fu, G., Fu G Fau - Dai, T., Dai T Fau - Huang, H. & H, H. - Migration of endothelial progenitor cells mediated by stromal cell-derived factor-1alpha/CXCR4 via PI3K/Akt/eNOS signal transduction pathway. J Cardiovasc Pharmacol 50, 274-280 (2007). 45 Ohtani, Y. et al. Expression of stromal cell-derived factor-1 and CXCR4 chemokine receptor mRNAs in cultured rat glial and neuronal cells. Neuroscience letters 249, 163-166 (1998). 46 Kollet O Fau - Shivtiel, S. et al. - HGF, SDF-1, and MMP-9 are involved in stress-induced human CD34+ stem cell recruitment to the liver. J Clin Invest 112, 160-169 (2003). 47 Sheu, M. L. et al. Recruitment by SDF-1alpha of CD34-positive cells involved in sciatic nerve regeneration. Journal of neurosurgery 116, 432-444, doi:10.3171/2011.3.jns101582 (2012). 48 Gleichmann, M. et al. Cloning and characterization of SDF-1gamma, a novel SDF-1 chemokine transcript with developmentally regulated expression in the nervous system. The European journal of neuroscience 12, 1857-1866 (2000). 49 Bain, J. R., Mackinnon, S. E. & Hunter, D. A. Functional evaluation of complete sciatic, peroneal, and posterior tibial nerve lesions in the rat. Plastic and reconstructive surgery 83, 129-138 (1989). 50 Detante, O. et al. Intravenous administration of 99mTc-HMPAO-labeled human mesenchymal stem cells after stroke: in vivo imaging and biodistribution. Cell transplantation 18, 1369-1379, doi:10.3727/096368909x474230 (2009). 51 Neuhaus, T. et al. Stromal cell-derived factor 1α (SDF-1α) induces gene-expression of early growth response-1 (Egr-1) and VEGF in human arterial endothelial cells and enhances VEGF induced cell proliferation. Cell Proliferation 36, 75-86, doi:10.1046/j.1365-2184.2003.00262.x (2003). 52 Salvucci O Fau - Yao, L. et al. - Regulation of endothelial cell branching morphogenesis by endogenous chemokine stromal-derived factor-1. Blood 99, 2703-2711 (2002). 53 Bonilla, C. et al. Failure of delayed intravenous administration of bone marrow stromal cells after traumatic brain injury. Journal of neurotrauma 29, 394-400, doi:10.1089/neu.2011.2101 (2012). 54 Ip, F. C., Cheung, J. & Ip, N. Y. The expression profiles of neurotrophins and their receptors in rat and chicken tissues during development. Neuroscience letters 301, 107-110 (2001). 55 Pitts, E. V., Potluri, S., Hess, D. M. & Balice-Gordon, R. J. Neurotrophin and Trk-mediated signaling in the neuromuscular system. International anesthesiology clinics 44, 21-76 (2006). 56 Sheard, P. W., Musaad, K. & Duxson, M. J. Distribution of neurotrophin receptors in the mouse neuromuscular system. The International journal of developmental biology 46, 569-575 (2002). 57 Clow, C. & Jasmin, B. J. Brain-derived neurotrophic factor regulates satellite cell differentiation and skeltal muscle regeneration. Molecular biology of the cell 21, 2182-2190, doi:10.1091/mbc.E10-02-0154 (2010). 58 Ernfors, P., Lee, K. F., Kucera, J. & Jaenisch, R. Lack of neurotrophin-3 leads to deficiencies in the peripheral nervous system and loss of limb proprioceptive afferents. Cell 77, 503-512 (1994). 59 Helgren, M. E. et al. Trophic effect of ciliary neurotrophic factor on denervated skeletal muscle. Cell 76, 493-504 (1994). 60 Marques, M. J. & Neto, H. S. Ciliary neurotrophic factor stimulates in vivo myotube formation in mice. Neuroscience letters 234, 43-46 (1997). 61 Rosen, J. M., Pham, H. N. & Hentz, V. R. Fascicular tubulization: a comparison of experimental nerve repair techniques in the cat. Annals of plastic surgery 22, 467-478 (1989). 62 Pan, H. C. et al. Neuroprotective effect of atorvastatin in an experimental model of nerve crush injury. Neurosurgery 67, 376-388; discussion 388-379, doi:10.1227/01.neu.0000371729.47895.a0 (2010). 63 Lapteva, N., Yang, A. G., Sanders, D. E., Strube, R. W. & Chen, S. Y. CXCR4 knockdown by small interfering RNA abrogates breast tumor growth in vivo. Cancer gene therapy 12, 84-89, doi:10.1038/sj.cgt.7700770 (2005). 64 Farrag Ty Fau - Lehar, M., Lehar M Fau - Verhaegen, P., Verhaegen P Fau - Carson, K. A., Carson Ka Fau - Byrne, P. J. & PJ, B. - Effect of platelet rich plasma and fibrin sealant on facial nerve regeneration in a rat model. Laryngoscope 117, 157-165 (2007).||摘要:||
背景:人類羊水間葉幹細胞（amniotic fluid mesenchymal stem cells：AFS），已經證實可以促進周邊神經再生。在神經受損後會表現基質衍生因子-1α(stromal derived factor 1α：SDF-1α)，SDF-1α可以藉由招募前趨細胞(progenitor cells)行使滋養功效(trophic effect)而促進神經細胞的修復。在本篇研究，我們探討在坐骨神經壓傷模式下，以不同時間點靜脈輸注受SDF-1α調節的羊水間葉幹細胞來評估神經修復的可行性。
材料與方法: 63隻Sprague-Dawley大鼠，使用血管夾造成左側坐骨神經壓傷。大鼠隨機分成三組：第一組：壓傷後注射生理食鹽水作為對照組；第二組：壓傷且在受傷後立即靜脈輸注羊水間葉幹細胞(每天給與5x106 cells共3天) (早期給與組)；和第三組：壓傷且在受傷第7天時靜脈輸注羊水間葉幹細胞(每天給與5x106 cells共3天) (晚期給與組)。在壓傷後每週評估神經行為、電生理研究、與修復標記(regeneration markers)。同時在不同時間點也評估羊水間葉幹細胞在各器官的分佈與SDF-1α及神經滋養因子(neurotrophic factor)的表現。
結果:在體外實驗藉由Wound healing assays與Transwell migration assay證實SDF-1α能促進羊水間葉幹細胞的移行，且細胞移行能力呈現劑量依賴性。無論是在神經或肌肉壓傷後皆能誘導SDF-1α的表現，且在第10-14天表現達到最高峰。 SDF-1α表現增加時，其受體Chemokine receptor type 4(CXCR-4)也一樣增加。不管在早期或晚期給與組，大部分羊水間葉幹細胞都分佈於肺部。只有在晚期給與組羊水間葉幹細胞明顯地沉積於神經和肌肉。在神經行為、電生理功能、神經組織髓鞘化及神經滋養因子和乙醯膽鹼接受體的表現，晚期給與組改善的程度優於其他兩組。
Background: Human amniotic fluid mesenchymal stem cells (AFS) have been shown to promote peripheral nerve regeneration. The expression of stromal derived factor 1α (SDF-1α) in the injured nerve exerts a trophic effect by recruiting progenitor cells that promote nerve regeneration. In this study, we investigated the feasibility of intravenous administration of AFS according to SDF-1α expression time profiles to facilitate neural regeneration in a sciatic nerve crush injury model.
Material and Methods: Peripheral nerve injury was induced in 63 Sprague-Dawley rats by crushing the left sciatic nerve using a vessel clamp. The animals were randomized into one of three groups: Group I: crush injury as the control; Group II: crush injury and intravenous administration of AFS (5x106 cells for 3 days) immediately after injury (early administration); and Group III: crush injury and intravenous administration of AFS (5x106 cells for 3 days) 7 days after injury (late administration). Evaluation of neurobehavior, electrophysiological study, and assessment of regeneration markers were conducted every week after injury. The expression of SDF-1α , neurotrophic factors, and the distribution of AFS in various time profiles were also assessed.
Results: SDF-1α increased the migration and wound healing of AFS in vitro, and the migration ability was dose dependent. Crush injury induced the expression of SDF-1α at a peak of 10-14 days either at nerve or muscle, and this increased expression paralleled the expression of its receptor CXCR-4. Most AFS was distributed to the lung during early or late administration. Significant deposition of AFS in nerve and muscle only occurred in the late administration group. Significantly enhanced neurobehavior, electrophysiological function, nerve myelination, and expression of neurotrophic factors and acetylcholine receptor were demonstrated in the late administration group.
Conclusion: AFS cells can be recruited by expression of SDF-1α in muscle and nerve after nerve crush injury. The increased deposition of AFS paralleled the expression profiles of SDF-1α and its receptor CXCR-4 either in muscle or nerve. AFS administration led to improvements of neurobehavior and expression of regeneration markers. Intravenous administration of AFS may be a promising alternative treatment strategy in peripheral nerve disorder.
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