Stem Cells International
Volume 2016 (2016), Article ID 7502178, 18 pages
http://dx.doi.org/10.1155/2016/7502178

Review Article

Using Stem Cells to Grow Artificial Tissue for Peripheral Nerve Repair

Kulraj Singh Bhangra,¹ Francesca Busuttil,² James B. Phillips,¹ and Ahad A. Rahim²

¹Department of Biomaterials and Tissue Engineering, UCL Eastman Dental Institute, University College London, 256 Gray’s Inn Road, London WC1X 8LD, UK
²Department of Pharmacology, UCL School of Pharmacy, University College London, 29–39 Brunswick Square, London WC1N 1AX, UK

Received 5 August 2015; Revised 17 February 2016; Accepted 2 March 2016

Academic Editor: Gerald A. Colvin

Copyright © 2016 Kulraj Singh Bhangra et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract.

Peripheral nerve injury continues to pose a clinical hurdle despite its frequency and advances in treatment. Unlike the central nervous system, neurons of the peripheral nervous system have a greater ability to regenerate. However, due to a number of confounding factors, this is often both incomplete and inadequate. The lack of supportive Schwann cells or their inability to maintain a regenerative phenotype is a major factor. Advances in nervous system tissue engineering technology have led to efforts to build Schwann cell scaffolds to overcome this and enhance the regenerative capacity of neurons following injury. Stem cells that can differentiate along a neural lineage represent an essential resource and starting material for this process. In this review, we discuss the different stem cell types that are showing promise for nervous system tissue engineering in the context of peripheral nerve injury. We also discuss some of the biological, practical, ethical, and commercial considerations in using these different stem cells for future clinical application.

1. Introduction

Despite advances in microsurgical techniques and a progressive understanding of pathophysiological mechanisms, peripheral nerve repair continues to be a major clinical challenge. Peripheral nerve injury (PNI) is often accompanied by loss of sensation, partial or complete apraxia, chronic pain, and occasionally permanent disability. Causes of peripheral nerve damage include conditions such as diabetes [1], Guillain-Barré syndrome [2], and cancer [3] along with iatrogenic injuries [4], but PNI prevails in the context of trauma [5]. Estimates vary, but approximately 300,000 cases of traumatic PNI present annually in Europe alone and in the United States PNI accounts for approximately 3% of all trauma cases and 5% if plexus and root avulsions are included [6, 7].

Peripheral nerves can regenerate to some extent and this ability is mainly attributable to intrinsic growth capacity of peripheral neurons and the ability of Schwann cells to provide a supportive growth environment [8]. Following a nerve transection injury, denervated Schwann cells in the distal part of the nerve adopt a regenerative phenotype and provide support to regenerating axons from the proximal stump. However, the degree of reinnervation is dependent on many factors such as the severity of injury, interstump gap length, alignment of nerve stumps, anatomical location of injury, delay before surgical intervention, and type of repair procedure applied [9]. In the case of chronic denervation, distal Schwann cells can lose their regenerative capacity, which can lead to incomplete regeneration [10, 11].

The clinical gold standard repair strategy for repairing large gaps in transected peripheral nerves is the nerve autograft. This offers a Schwann cell-rich autologous material to bridge the interstump gap and serves to guide regenerating axons. This method is not ideal because of donor site morbidity, the requirement for additional surgery, and limited donor tissue availability. The limitations of autografting have led to the search for alternative therapies. In particular, the use of tissue engineering to construct artificial tissue that mimics the nerve autograft provides a potentially innovative solution for peripheral nerve repair. Various authors have reviewed natural and synthetic materials for nerve tissue engineering [12–15] so the aim of this review is to explore the cellular components that could be used in an engineered tissue to encourage nerve regeneration. Since the use of allogeneic Schwann cells requires a source of nerve tissue, it is affected by the same factors that limit the autograft. This has resulted in the development of a range of approaches that use stem cells as a source of therapeutic material.

The ability of stem cells to self-renew and to differentiate towards a desired lineage makes them a popular choice as the starting point for cell therapies. Nevertheless, there are issues regarding host immune response after administration, oncogenic properties that give rise to teratomas or teratocarcinomas, in addition to various ethical concerns [16, 17]. This review discusses recent studies in which stem cells have been used as sources of therapeutic cells to construct artificial peripheral nerve tissue. It also considers the practicalities associated with different sources of therapeutic cells in terms of biological and commercial feasibility for translation to the clinic.

2. Preclinical Studies Using Stem Cells for Peripheral Nerve Repair

The inclusion criteria for the studies in Table 1 included (1) in vivo experimental study in animals or humans, (2) use of a nerve conduit or graft as a scaffold for stem cell delivery, and (3) studies within the last 5 years (2010–2015). The exclusion criteria included (1) in vitro experimental studies, (2) use of injection as a mode of delivery of the stem cells, and (3) models of crush injuries, that is, absence of a gap between the proximal and distal stumps of the injured nerve.

Table 1: Summary of current evidence assessing the effect of different stem cell types on peripheral nerve regeneration in animal models.

Stem cell source tissue
Author
Experimental model
Mode of delivery
Therapeutic cell properties
Key outcome measures

Adipose
Georgiou et al. [99]
Rat sciatic transection (15 mm gap, 8 weeks)
Aligned cellular collagen constructs in a collagen tube
Differentiated rat ADSCs
Axon regeneration, myelination.

Hsueh et al. [185]
Rat sciatic transection (10 mm gap, 6 weeks)
Neurospheres seeded in a chitosan-coated silicon conduit
Xenogeneic hADSC neurospheres
Axon regeneration, myelination, inflammation, intraneural scarring, muscle fibres, and gait.

Kingham et al. [97]
Rat sciatic transection (10 mm gap, 2 weeks)
Cells in fibrin matrix seeded in a fibrin conduit
Stimulated xenogeneic hADSCs
Axon regeneration, vascularisation, cell survival, and gene expression changes in DRG and spinal cord.

Scholz et al. [186]
Athymic rat sciatic transection (13 mm gap, up to 4 months)
Cells in culture medium seeded in a silastic conduit
Xenogeneic differentiated hADSCs
Axon regeneration, extensor postural thrust, sensory evaluation, and muscle weight.

Carriel et al. [187]
Rat sciatic transection (10 mm gap, 12 weeks)
Cells in a fibrin-agarose hydrogel seeded in a collagen conduit
Autologous ADSCs
Axon regeneration, myelination, electrophysiology, pinch test, and toe spread.

Mohammadi et al. [33]
Rat sciatic transection (10 mm gap, up to 12 weeks)
Cells in PBS seeded in a silicone conduit
Allogeneic ADSCs
Nerve fibres, walking track analysis, and muscle weight.

Suganuma et al. [188]
Rat sciatic transection (10 mm gap, 2 weeks)
Cells in type I collagen gel seeded in a silicone conduit
Autologous uncultured ADSCs
Axon regeneration, Schwann cell infiltration, cell survival, and gene expression in repaired tissue.

Orbay et al. [189]
Rat sciatic transection (10 mm gap, up to 6 months)
Cells in collagen gel seeded in a silicone conduit
Autologous ADSCs differentiated into Schwann cell-like cells
Nerve fibres, vascularisation, cell survival, walking track analysis electrophysiology, and muscle weight.

Liu et al. [190]
Rat sciatic transection (15 mm gap, 12 weeks)
Cells in culture medium seeded in an acellular nerve allograft
Allogeneic undifferentiated ADSCs
Footprint analysis, sciatic functional index, electrophysiology, myelination, and nerve fibre density.

Reid et al. [191]
Rat sciatic transection (10 mm gap, 2 weeks)
Cells in culture medium seeded in a PCL conduit
Allogeneic ADSCs differentiated into Schwann cell-like cells
Gene expression changes in the DRG.

Shen et al. [192]
Rat sciatic transection (10 mm gap, up to 8 weeks)
Cells in culture medium seeded in a GGT conduit
Allogeneic undifferentiated ADSCs
Electrophysiology, walking track analysis, footprint analysis, nerve fibres, and myelination.

Sun et al. [193]
Rat facial transection (8 mm gap, 8 weeks)
Cells in culture medium seeded in a decellularised allogeneic artery conduit
Autologous ADSCs differentiated into Schwann cell-like cells
Functional evaluation of vibrissae movement, electrophysiology, morphological evaluation of regenerated nerve segments, and retrograde labelling of facial motor neurons.

Wei et al. [194]
Rat sciatic transection (10 mm gap, up to 24 weeks)
Cells in culture medium seeded onto a chitosan/silk fibroin conduit
Allogeneic undifferentiated ADSCs
Walking track analysis, footprint analysis, muscle mass, axon regeneration, and myelination.

di Summa et al. [93]
Rat sciatic transection (10 mm gap, 2 weeks)
Cells in culture medium seeded in a fibrin conduit
Allogeneic ADSCs differentiated into Schwann cell-like cells
Axon regeneration, Schwann cell infiltration.

Erba et al. [94]
Rat sciatic transection (10 mm gap, 2 weeks)
Cells in fibrinogen seeded in a PHB conduit
Allogeneic undifferentiated ADSCs
Axonal regeneration, transplanted cell tracking.

Zhang et al. [195]
Rat sciatic transection (10 mm gap, 3 months)
Cells in culture medium seeded in a xenogeneic acellular graft
Autologous ADSCs differentiated to a neuronal phenotype
Axon regeneration, myelination, and electrophysiology.

Ghoreishian et al. [196]
Dog facial nerve transection (7 mm gap, 12 weeks)
Cells in an alginate hydrogel seeded in a GORE-TEX® conduit
Autologous undifferentiated ADSCs
Axon regeneration, electrophysiology.

Bone marrow
Ding et al. [36]
Dog sciatic transection (50 mm gap, 6 months)
Cells in culture medium seeded in a chitosan/PLGA conduit
Autologous undifferentiated BMSCs
Electrophysiology, muscle mass, axon regeneration, myelination, and vascularisation.

Xue et al. [37]
Dog sciatic transection (60 mm gap, 12 months)
Cells in saline seeded in a chitosan/PLGA conduit
Autologous undifferentiated BMSCs
Posture and gait analysis, electrophysiology, muscle mass, myelination, and nerve fibres.

Sakar et al. [197]
Rat sciatic transection (10 mm gap, up to 8 weeks)
Cells in PBS seeded in a PHBHHx nerve graft
Allogeneic undifferentiated BMSCs
Electrophysiology, axon regeneration, myelination, walking track analysis, and vascularisation.

Hu et al. [38]
Monkey median transection (50 mm gap, 1 year)
Cells in culture medium seeded in a chitosan/PLGA conduit
Autologous undifferentiated BMSCs
Behaviour observation, electrophysiology, myelination, safety evaluation, and axon regeneration.

Wakao et al. [39]
Monkey median transection (20 mm gap, 1 year)
Cells in a collagen sponge seeded in a biodegradable conduit
Autologous BMSCs differentiated to Schwann cell-like cells
Cell proliferation for local tumour formation, electrophysiology, hand movement analysis, immunocytochemistry, general health follow-up, immune response, myelination, and axon regeneration.

Oliveira et al. [156]
Mouse median transection (2 mm gap, 8 weeks)
Cells in culture medium seeded in a PCL conduit
Autologous undifferentiated BMSCs
Myelination, nerve fibres, electrophysiology, muscle mass, creatine phosphokinase levels, grasping test, and immunohistochemistry.

Ladak et al. [34]
Rat sciatic transection (12 mm gap, 12 weeks)
Cells in culture medium seeded in a biodegradable collagen nerve guide
Autologous BMSCs differentiated to Schwann cell-like cells
Electrophysiology, axon regeneration, and muscle mass.

Mohammadi et al. [198]
Rat sciatic transection (10 mm gap, up to 12 weeks)
Cells in PBS seeded in an inside-out vein graft
Allogeneic undifferentiated BMSCs
Walking track analysis, immunohistochemistry, muscle mass, axon regeneration, and myelination.

Embryonic
Cui et al. [28]
Rat sciatic transection (10 mm gap, up to 3 months)
Cells in culture medium seeded into the gap between the nerve stumps with the surrounding epineurium as a natural conduit
Xenogeneic mouse ESCs differentiated into neural progenitor cells
Electrophysiology, axon regeneration, and myelination.

Umbilical cord (Wharton’s Jelly)
Matsuse et al. [102]
Rat sciatic transection (8 mm gap, up to 21 days)
Cells in Matrigel seeded in transpermeable tubes
Allogeneic umbilical cord stem cells differentiated into Schwann cell-like cells
Walking track analysis, immunohistochemistry, myelination, and axonal regeneration.

Dental pulp
Matsushita et al. [199]
Rat sciatic transection (3 mm gap, up to 32 weeks)
Cells in PBS seeded in a chitosan conduit
Xenogeneic human whole dental pulp
Immunohistochemistry, myelination, and axon regeneration.

Neural tissue
Ni et al. [80]
Rat sciatic transection (15 mm gap, up to 12 weeks)
Cells in culture medium seeded in a PLA conduit
Xenogeneic mouse undifferentiated NSCs
Walking track analysis, sciatic functional index, electrophysiology, revascularisation, axon regeneration, and myelination.

Liard et al. [79]
Pig femoral transection (30 mm gap, up to 240 days)
Neurospheres seeded in an autologous venous bridge
Allogeneic undifferentiated NSCs
Electromyography, thigh flexion, and phenotypic characterization of grafted cell progeny.

Skin
Park et al. [73]
Pig femoral transection (10 mm gap, up to 4 weeks)
Cells in fibrin glue seeded in a Lyoplant® conduit
Autologous undifferentiated SKPs
Axon regeneration, nerve fibres.

iPSCs
Uemura et al. [86]
Mouse sciatic transection (5 mm gap, up to 48 weeks)
Neurospheres seeded in a PCL/PLA conduit
Mouse iPSCs differentiated to neurospheres
Print length factor, foot withdrawal, histomorphometry, and myelination.

Wang et al. [45]
Rat sciatic transection (10 mm gap, 1 month)
Cells in Matrigel seeded in a PCL/PLA/sodium acetate conduit
Human iPSCs differentiated to neural crest stem cells
Myelination, axon regeneration, electrophysiology, and cell survival.

ADSCs: adipose derived stem cells; hADSCs: human adipose derived stem cells; DRG: dorsal root ganglion; PBS: phosphate buffered saline; PCL: poly-ε-caprolactone; GGT: genipin cross-linked gelatin annexed with tricalcium phosphate ceramic particles; PHB: poly-3-hydroxybutyrate; PLGA: poly(lactic-co -glycolic acid); BMSCs: bone marrow stem cells; PHBHHx: poly(3-hydroxybutyrate-co-3- hydroxyhexanoate); ESCs: embryonic stem cells; PLA: polylactic acid; NSCs: neural stem cells; SKPs: skin derived precursors; iPSCs: induced pluripotent stem cells.

3. Sources of Stem Cells Used in Nerve Tissue Engineering

3.1. Embryonic Stem Cells (ESCs)

In 1998, Thomson et al. [18] described the isolation of a pluripotent cell line from the human blastocyst. The use of ESCs to treat CNS disorders is well-documented [19–21], while it seems their potential to treat PNS injuries remains largely unexplored. Due to their pluripotency, differentiation along a specific neural lineage is challenging [22]. A study by Ziegler et al. [23] generated neurospheres from hESC by coculture with stromal cells, grown under conditions supportive of Schwann cell differentiation. After 8 weeks, hESCs differentiated into cells with morphological and molecular features characteristic of Schwann cells and associated with neurites from chick, rat, and human origin in vitro. Various other studies have shown that ESC can differentiate along a neural lineage [24–27].

Cui et al. [28] injected mouse ESCs into a sciatic nerve in a rat axotomy model (after the sciatic nerve was transected, the surrounding epineurium was resutured). ESCs were neurally induced and were transplanted 1 hour after removal of a 10 mm segment of nerve. Three months following axotomy, the ESCs survived and Fluoro-Gold (FG) retrograde staining along with electrophysiology showed better regeneration than controls.

Several groups have reported that ESCs share behavioural characteristics similar to cancer cells and express markers that are also found in many human and mouse cancer models [29, 30]. Undifferentiated ESCs have been known to form teratomas or teratocarcinomas [31]. In addition, there are risks of immunogenicity and various ethical barriers presented by this stem cell source [16].

3.2. Bone Marrow Stem Cells (BMSCs)

Several in vitro studies have reported that BMSCs can be induced to differentiate into neural lineages including neurons, astrocytes, oligodendrocytes, and Schwann-like cells [32]. Experimental studies in rats [33, 34], rabbits [35], dogs [36, 37], and primates [38, 39] have investigated the effectiveness of these cells in improving functional outcomes following peripheral nerve repair. Wang et al. [40] suggested that rat BMSCs can positively influence the regeneration of peripheral nerves not only through the direct release of neurotrophic factors, but also through indirect modulation of the behaviour of Schwann cells.

Caddick et al. [41] demonstrated that rat BMSCs can be differentiated into cells that are Schwann cell-like in both phenotype and function. Following differentiation with all-trans-retinoic acid (ATRA), platelet derived growth factor (PDGF), basic fibroblast growth factor (BFGF), and forskolin, BMSCs underwent morphological changes to resemble cultured Schwann cells and stained positive for the Schwann cell markers S100, P75, and glial fibrillary acidic protein (GFAP). The differentiated BMSCs were also found to enhance neurite outgrowth in coculture with sensory neurons to a level equivalent or superior to that produced by Schwann cells. Further reports indicating that differentiated BMSCs can mimic the functions of Schwann cells in culture have since been published [34, 42, 43].

Keilhoff et al. [44] showed that rat BMSCs can be differentiated in vitro into Schwann-like cells using a combination of cytokines. The myelinating capacity of the transdifferentiated cells was studied in coculture with PC12 cells and by grafting into an autologous muscle conduit bridging a 2 cm gap in a rat model. In vitro, transdifferentiated BMSCs were able to myelinate PC12 cells after 14 days while, in vivo, they increased the numbers of newly myelinated fibres after 3 weeks.

Autologous transdifferentiated BMSCs were transplanted into a monkey model of median nerve injury using a polymer tube containing a collagen sponge [39]. This study showed improvements in behaviour, electrophysiology, and histology for up to one year. Further studies have shown that the addition of BMSCs to conduits and acellular grafts results in superior outcomes when compared with empty channels [37, 38, 45, 46]. Furthermore, the nerve regeneration capacity of BMSCs can be dose dependent, as indicated by Raheja et al. [47], who reported better improvements in rats with a sciatic nerve transection treated with a high dose of cells compared to those treated with a low dose and controls.

3.3. Skeletal Muscle Derived Stem Cells (SMDSCs)

Tamaki et al. [48] reported that skeletal muscle interstitium contained multipotent stem cells. It was further established that these were able to differentiate into mesodermal cells (including skeletal muscle cells and endothelial cells) and ectodermal cells such as Schwann cells and perineurial cells in vivo [49]. In addition to multipotent differentiation, SMDSCs are characterized by sustained self-renewal and long-term proliferation [50]. Another potentially favourable characteristic of these cells is their survival capability under conditions of oxidative and hypoxic stresses [51].

In another study, Tamaki et al. [52] utilised a nerve crush injury model in mice to examine the differentiation capacity and contributions of undifferentiated murine SMDSCs in peripheral nerve regeneration. After 4 weeks, engrafted SMDSCs differentiated into Schwann cell-like cells which myelinated the regenerated axons. Additionally, the SMDSCs were reported to form perineurial/endoneurial cells and associated blood vessels composed of donor-derived endothelial cells, pericytes, and fibroblasts. Facilitated nerve regeneration and improved walking function was also observed when SMDSCs were applied to an acellular conduit to enhance nerve gap bridging in the same study.

Lavasani et al. [53] used human SMDSCs to repair a critical-sized sciatic nerve injury in a mouse model. Transplanted human SMDSCs surrounded the axonal growth cone, while those infiltrating the regenerating nerve differentiated into myelinating Schwann cells. Engraftment of human SMDSCs into the area of the damaged nerve promoted axonal regeneration, which led to functional recovery as measured by sustained gait improvement. Furthermore, no adverse effects were reported in these animals up to 18 months after transplantation. Following human SMDSC therapy, gastrocnemius muscles from mice exhibited substantially less muscle atrophy, an increase in muscle mass after denervation, and reorganization of motor endplates at the postsynaptic sites compared with those from control mice.

3.4. Dental Pulp Stem Cells (DPSCs)

The dental pulp contains connective tissue, mesenchymal cells, neural fibres, blood vessels, and lymphatics [54] as well as DPSCs that can self-renew and undergo multidifferentiation [55]. Due to their neural crest origin (in common with cells forming the peripheral nervous system) [56], DPSCs may be more amenable to neural and glial cell differentiation than other stem cell sources [57]. In fact, even in an undifferentiated state, human DPSCs in vitro expressed markers such as S100 and nerve growth factor receptor p75 and were able to produce and secrete a range of neurotropic factors including vascular endothelial growth factor (VEGF), brain-derived neurotrophic factor (BDNF), and glial-derived neurotrophic factor (GDNF) [58]. This makes DPSCs an attractive candidate for the treatment of PNI [59].

Sasaki et al. [60] used a silicone tube containing a collagen gel embedded with rat dental pulp cells to repair a gap in the rat facial nerve. Twelve days after transplantation, defective facial nerves connected with silicone tubes containing dental pulp cells were able to support axonal growth to a greater extent than with tubes containing the collagen gel alone. The regenerated nerves contained myelinated fibres and retrograde tracing demonstrated the presence of Fluoro-Gold-positive motor neurons in the facial nucleus of the rat brain. Although this work was undertaken with dental pulp cells as a mixed population, rather than isolated DPSCs, it illustrates the potential of DPSCs in peripheral nerve regeneration.

In a more recent study, Martens and colleagues [58] evaluated the potential of human DPSCs to differentiate towards a Schwann cell lineage. Schwann cell differentiation was examined at the morphological and ultrastructural level and the differentiated human DPSCs showed glial marker expression and secreted neurotrophic factors that promoted sensory neuron survival and neurite outgrowth in vitro. In addition, neurites were myelinated by the differentiated human DPSCs in an aligned 3-dimensional coculture system and an engineered neural tissue construct containing aligned human DPSCs in stabilised collagen hydrogels further supported and guided neurite outgrowth.

3.5. Hair Follicle Stem Cells (HFSCs)

Stem cells from hair follicles are attractive candidates for use in cell therapy [61], and different populations of HFSCs have been identified [62–64].

Li et al. [62] reported nestin-expressing stem cells in the bulge area of hair follicles which were subsequently shown to be able to differentiate into various nonfollicle cell types and are now known as hair follicle-associated pluripotent stem cells [65]. Mouse green fluorescent protein positive HFSCs were implanted into the gap region of a severed sciatic nerve in a mouse model [66]. The HFSCs differentiated largely into Schwann cells, which produced myelin sheaths around the host axons. Function of the repaired sciatic nerve was measured by contraction of the gastrocnemius muscle upon electrical stimulation. Additionally, HFSCs were implanted in the gap of a severed tibial nerve in a mouse model, resulting in improved walking outcome measures. In a more recent study by Amoh et al. [67], human HFSCs were transplanted around the impinged sciatic nerve in a mouse model, where they differentiated into GFAP-positive cells that associated with host axons. Eight weeks after the transplantation of human HFSCs, gastrocnemius muscle contraction was recorded upon electrical stimulation of the repaired sciatic nerves. Lin et al. [68] differentiated rat HFSCs into Schwann cells in vitro using NRG1. These cells, together with neurons, were injected into a decellularised scaffold and cultured in vitro. Survival and proliferation of seeded cells as well as neuron-Schwann cell contacts in the scaffolds were observed for at least eight weeks.

Recently, Sakaue and Sieber-Blum isolated human epidermal neural crest stem cells from the hair follicle bulge and showed they can be differentiated into functional Schwann cells [69]. Manipulation of WNT, sonic hedgehog, and tumour-growth-factor β signalling pathways and exposing the cells to growth factors led to the expression of Schwann cell markers. Further gene expression profiling indicated the expression of neurotropic and angiogenic transcripts, making these cells promising candidates for nerve repair.

3.6. Skin Derived Precursors (SKPs)

Toma et al. [70] reported that multipotent adult stem cells isolated from mammalian dermis can proliferate and differentiate in culture to produce neurons, glia, smooth muscle cells, and adipocytes. SKPs exhibit many similarities to embryonic neural crest stem cells (NCSCs) [71]. McKenzie et al. [72] differentiated SKPs into Schwann cells using medium containing forskolin and NRG1. The Schwann cells were able to proliferate and to express myelin proteins in coculture with sensory neurons. Following transplantation into a mouse sciatic crush model, SKPs associated with and myelinated the host axons within six weeks.

Park et al. [73] investigated the in vivo peripheral nerve regeneration potential of autologous porcine SKPs in fibrin glue and collagen tubes following transplantation into a femoral nerve defect miniature pig model. The transplanted cells survived for at least four weeks and histologically complete nerve bundles were observed in the regenerated nerve tissues. Additionally, higher levels of S100 and p75 were detected in the treated animals than in the controls. Khuong et al. [74] studied the effects of SKPs on acute and chronic nerve repair as well as a nerve gap injury repaired with a nerve graft in rats. When used as an adjunct to standard microsurgical nerve repair, SKPs improved outcome in all three scenarios.

A novel case report by Grimoldi et al. [75] used a collagen tube filled with autologous skin derived stem cells to repair the motor and sensory nerves of the left arm of a 23-year-old female patient. Motor and sensory functions of the median nerve demonstrated ongoing recovery after implantation during the three-year follow-up period. Functional recovery of injured median and ulnar nerves was assessed by pinch gauge test and static two-point discrimination and touch test with monofilaments, along with electrophysiological and magnetic resonance imaging (MRI) examinations.

3.7. Neural Stem Cells (NSCs)

NSCs have been isolated from both the embryonic and the adult central nervous system [76–78]. Liard et al. [79] transplanted adult pig subventricular zone NSCs inside an autologous venous graft into a femoral nerve gap in an adult pig model and reported improved functional recovery at 6 months compared to controls. Postmortem immunohistochemistry revealed neurosphere-derived cells that survived inside the venous graft from 10 to 240 days and all displayed a neuronal phenotype. Moreover, NSC transplantation increased 2′,3′-cyclic nucleotide 3′-phosphodiesterase (CNPase) expression, indicating activation of intrinsic Schwann cells.

Ni et al. [80] utilised poly(D, L-lactic acid) (PLA) conduits with immobilized fibroblast growth factor 1 (FGF1) and seeded with adult mouse NSCs to bridge a critical size sciatic nerve gap in a rat model. Axon regeneration and functional recovery were observed and evaluated by histology, walking track analysis, and electrophysiology for up to 12 weeks after implantation. In a recent study by Jenkins and colleagues [81], human NSCs were induced from embryonic stem cells and were cultured on an electrospun nerve guidance conduit to evaluate its ability to promote neuronal growth and axonal extension. NSCs survival, migration, and guided neurite extension were observed.

Fu et al. [82] used two recombinant mammalian vectors containing either rat GDNF gene or BDNF gene to transfect adult mouse NSCs. The transfected NSCs showed significantly enhanced expression of GDNF or BDNF mRNA. The transfected NSCs were seeded onto a PLA conduit and implanted into a rat model of sciatic nerve transection. Improved regeneration, myelination, and functional recovery were associated with conduits seeded with the transfected NSCs.

Johnson et al. [83] implanted C17.2 cells, an immortalized mouse NSC line, into three different sciatic nerve injury rat models. Twelve of the forty-five animals used in the study developed large tumours resembling neuroblastomas at the site of the NSC transplants, precluding meaningful interpretation of functional outcome or muscle mass preservation in either the sciatic nerve transection and repair or the crush injury models. The tumour formation was thought to occur as a result of the accumulation of growth factors secreted in high concentrations by the C17.2 cells. Additionally, the transplanted NSCs themselves could have undergone excessive proliferation without the desired differentiation. The authors suggest that further characterization of the interaction of these cells with surrounding tissues of the peripheral nervous system has to be carried out before clinical translation of this approach.

3.8. Induced Pluripotent Stem Cells (iPSCs)

Takahashi and Yamanaka [84] used four transcription factors, namely, Oct3/4, Sox2, c-Myc, and Klf4, to generate pluripotent cells, subsequently called iPSCs directly from mouse embryonic or adult fibroblast cultures. Parameters such as factor stoichiometry and culture medium and supplementation have been demonstrated to affect the quality of the iPSCs produced [85].

Wang et al. [45] derived neural crest stem cells from human iPSCs and embryonic stem cells. The neural crest stem cells were seeded into nanofibrous tubular scaffolds (electrospun poly(L-lactide-co-caprolactone)) and used as a bridge for transected sciatic nerves in a rat model. Electrophysiological analysis showed that neural crest stem cell-engrafted nerve conduits resulted in an accelerated regeneration of sciatic nerves at one month when compared with controls. Histological analysis demonstrated that neural crest stem cell transplantation resulted in differentiation into Schwann cells that were able to myelinate the host axons. No teratoma formation was observed for up to one year after neural crest stem cell transplantation in vivo. Similar results were obtained by Uemura et al. [86] who examined the long-term outcome of transplanting iPSC-derived neurospheres within nerve conduits for peripheral nerve repair in mice. They confirmed that no teratoma formation was observed up to 48 weeks after transplantation, and axonal regeneration and myelination were enhanced.

Ikeda et al. [87] attempted to repair a sciatic nerve defect in a mouse model by using a bioabsorbable nerve conduit containing both iPSC-derived neurospheres and a basic fibroblast growth factor delivery system. The iPSCs were cultured and differentiated into primary neurospheres containing neural stem cells then secondary neurospheres, which according to Nori et al. [88] differentiated mainly into glial lineage cells. Axon regeneration and functional recovery in the mice were reported to be improved 12 weeks after reconstruction when this combination approach was used.

The derivation of iPSCs from somatic cells provides much potential for patient-specific cell therapies, which bypasses immune rejection issues and ethical concerns associated with using embryonic stem cells as a cell source. However, many important issues need to be addressed in order to use iPSCs in neural tissue engineering, such as differences among iPSC populations in differentiation and expansion and the appropriate differentiation stage of the cells for specific tissue engineering applications [45].

3.9. Adipose Derived Stem Cells (ADSCs)

Adipose tissue is largely comprised of adipocytes as well as a smaller stromal vascular fraction which includes ADSCs [89]. These mesenchymal stem cells can be isolated and have been shown to differentiate into cell types of all three germ layers in vitro [90, 91]. ADSCs have been extensively studied as an adjunct to nerve repair [92].   

di Summa et al. [93] compared adult rat ADSCs and BMSCs each differentiated to a Schwann cell-like phenotype for the repair of a sciatic nerve injury in a rat model. The mesenchymal stem cells were differentiated into Schwann cell-like cells using a combination of PDGF, BFGF, forskolin, and NRG1. The resulting Schwann cell-like cells from both sources enhanced regeneration but, unlike BMSCs, ADSCs can be harvested less invasively with a higher yield and can be rapidly expanded in vitro and show low immunogenicity [92]. 

Erba et al. [94] investigated the ability of undifferentiated rat ADSCs in a poly-3-hydroxybutyrate nerve conduit to enhance axonal growth as well as their ability to differentiate in situ in a rat sciatic transection model (10 mm gap, 2 weeks). The ADSCs increased regeneration and Schwann cell proliferation compared to controls. However, 14 days after transplantation, a lack of viable implanted cells was observed. As a result, the authors were unable to detect any in situ differentiation of ADSCs into neuronal or glial cell types. Similar results were obtained by Santiago et al. [95], who reported that while the transplantation of human ADSCs in a rat sciatic nerve defect promoted nerve tissue regeneration and a decrease in muscle atrophy, the ADSCs did not differentiate to Schwann cell-like cells at the site of injury. This suggests that the regenerative effect of transplanted ADSCs is likely due to an initial boost of released growth factors as well as an indirect effect on endogenous Schwann cell activity. Further evidence for peripheral nerve regeneration through the paracrine effects of ADSCs is presented by Widgerow et al. [96] and Kingham et al. [97]. 

Tomita et al. [98] differentiated human ADSCs into Schwann cell-like cells and transplanted them into a rat model of tibial nerve crush, where they closely associated with host axons. The presence of myelin basic protein was detected 8 weeks after transplantation and improved myelin formation was observed with the Schwann cell-like cells compared with undifferentiated ADSCs.  In a recent study, Georgiou et al. [99] used differentiated rat adipose derived stem cells to construct engineered neural tissue through a combination of cellular self-alignment and plastic compression in a collagen hydrogel. The sheets of aligned cellular collagen supported axon regeneration over a critical length gap (15 mm, 8 weeks) in rat sciatic nerves. Interestingly, the phenotype of the differentiated ADSCs changed when they were transferred to the three-dimensional collagen environment from cell culture flasks, with an apparent increase in expression of key growth factors associated with the support of regeneration.

3.10. Perinatal Stem Cells

Perinatal tissues are a potentially useful source of stem cells for tissue engineering purposes as they can be collected in great numbers without causing harm to the donor. Multipotent stem cells have been derived from the placenta, amniotic fluid, amniotic membrane, and umbilical cord [100]. Foetal tissue age rarely exceeds 42 weeks and therefore, in comparison to adult sources, perinatal cells can have less accumulated genetic damage [101].

Matsuse et al. [102] induced human umbilical cord mesenchymal stem cells (UC-MSCs) to differentiate into Schwann cell-like cells then seeded these in transpermeable tubes and transplanted into transected sciatic nerves in adult rats. The Schwann cell-like cells reportedly myelinated the regenerated axons and promoted functional recovery for 21 days after transplantation. Similar results were also obtained by Kuroda et al. [103] and Pereira et al. [104]. In addition to differentiating to a Schwann cell phenotype and expressing Schwann cell markers, Peng and colleagues [105] reported that Schwann cell-like cells derived from human UC-MSCs released BDNF, NGF, and neurotrophin-3 in vitro. When these cells were cocultured with PC12 cells, neurite outgrowth was observed.

Pan et al. [106] evaluated the effects of neurotrophic factors secreted by rat amniotic fluid mesenchymal stem cells on regeneration of sciatic nerve after crush injury in a rat. Rat amniotic fluid mesenchymal stem cells were embedded in fibrin glue and wrapped around the injured nerve in woven Surgicel®. High levels of expression of BDNF, GDNF, ciliary neurotrophic factor, NGF, and neurotrophin-3 were demonstrated in the amniotic fluid mesenchymal stem cells. Motor function recovery, compound muscle action potential, and nerve conduction latency showed significant improvement in rats treated with amniotic fluid mesenchymal stem cells. Additionally, a high level of expression of S100 and GFAP was observed at the crush site. Similar results were obtained by Li et al. [107] who transplanted amniotic stem cells into a mouse model of a crushed sciatic nerve. Additionally they reported that the stem cells augmented blood perfusion, increased intraneural vascularity, and localised to the perineurium.

4. Clinical Translation of Stem Cells: Insights for Peripheral Nerve Repair

4.1. Stem Cells Used in Active Clinical Trials

As of July 2015, the clinical trials database (https://clinicaltrials.gov/) showed 117 clinical trials using human stem cells internationally and 11 of those trials had reached Phase III and Phase IV status (Figure 1). Of these 11, umbilical cord blood stem cells are the most common source (8 trials) followed by adipose derived stem cells, neural stem cells, and epithelial stem cells (1 trial of each). Cogle et al. [108] and G. D. Fischbach and R. L. Fischbach [109] have reviewed the underlying regulatory, ethical and legal barriers to clinical translation of stem cells and more specifically Walsh and Midha [110] have discussed the practical considerations of using stem cells for peripheral nerve repair.

Figure 1: Summary of active (nonrecruiting) clinical trials using stem cell sources internationally. The search was performed on the website of ClinicalTrials.gov (https://clinicaltrials.gov/) on July 28, 2015, and results show there are 117 active studies (a) with 11 studies currently in Phase III or Phase IV clinical trials. Keywords included “Bone marrow derived stem cells” (), “Adipose derived stem cells” (), “Dental pulp stem cells” (), “Neural stem cells” (), “Skin derived stem cells” (), “Epithelial derived stem cells” (), “Umbilical cord blood stem cells” (), “Embryonic stem cells” (), and “Induced pluripotent stem cells” (). With regard to the Phase III and Phase IV trials (b) umbilical cord blood stem cells are the most common stem cells sources () followed by adipose derived stem cells (), neural stem cells (), and epithelial stem cells ().

4.2. Regulatory Considerations

Currently, there are no licensed stem cell based artificial nerve tissues for peripheral nerve repair. Using stem cells in clinical trials requires formal approval by the relevant regulatory bodies that are responsible for ensuring that therapies meet standards of safety and quality without jeopardising public health and national security. Berger et al. [111] have recently compared regulatory frameworks with regard to stem cell-based therapies. Their review shows that USA and Europe have the largest number of clinical trials using stem cells followed by East Asia. More notably, since the discovery of induced pluripotent stem cells [84], Japan, which has a similar regulatory framework to USA and Europe, has refined its guidelines to push forward the development of stem cell innovations and has led to the first-ever clinical trial using iPSCs [112].

In Europe, the European Medicines Agency (EMA) regulates stem cell-based therapies and related tissue-engineered medicinal products such as those developed for peripheral nerve repair. Such cellular constructs would be regulated as Advanced Therapy Medicinal Products (ATMPs) [113]. In the UK, the Medicines Health and Regulatory Agency (MHRA) is the competent authority responsible for ATMPs and related clinical trials. For an ATMP to achieve regulatory approval in Europe it would be subject to a centralized marketing procedure whereby applications would be assessed by the Committee for Advanced Therapies and the Committee for Medicinal Products for Human Use before a decision is made by the EMA to grant or refuse marketing authorisation.

In the USA, stem cells and tissue-based devices are regulated by the Food and Drug Administration (FDA) as Human Cells and Tissue-Based Products (HCT/Ps). For peripheral nerve repair application, cells are often combined with natural or synthetic materials to form artificial nerve tissue and are classified as “biological drugs.” These are regulated by the Center for Biologics Evaluation and Research. Whether it be for clinical trials or commercialising a product such as artificial nerve tissue constructs, authorisation must be sought from the FDA through submission of a Biologics License Application. The regulatory framework for Japan is similar to that of Europe and USA [111] and guidelines governing the translation of stem cell therapies were established by the Ministry of Health, Labor and Welfare (MHLW). Kawakami et al. [114] discuss the regulatory impacts of stem cell research in Japan; however, currently a specific framework regulating tissue-engineered products does not exist.

Japan has recently passed a Regenerative Medicine Promotion Law, which provides the opportunity for patients to be treated with regenerative therapies based on the latest scientific knowledge, thus permitting earlier patient access. Further details about the new regulatory system for stem cell therapies in Japan have recently been reviewed by Hara and colleagues [115]. The USA have also introduced schemes to accelerate the delivery of stem cell-based therapies such as “Fast Track,” “Breakthrough Therapy,” “Accelerated Approval,” and “Priority Review” [116] and Knoepfler [117] thoroughly reviews emerging regulatory trends for new stem cell therapies in the USA. Another regulatory pathway for earlier patient access has recently been proposed by Caplan and West [118]. Such schemes to provide earlier patient access are also gaining traction in Europe via the adaptive pathway approach. March of 2014 saw the EMA inviting companies to participate in pilot project adaptive pathways aiming at well-defined patient groups with serious conditions and unmet medical needs [119].

4.3. Manufacture and Cell Processing

Obtaining formal approval for a clinical trial from the aforementioned regulatory bodies requires aligning manufacture and cell processing with current Good Manufacturing Practice (GMP), Good Tissue Practice, and Good Clinical Practice. The practice guidelines encompass everything from procurement of stem cells to assessing long-term feasibility and scalability.

A key regulatory issue to consider in the development of stem cell-based therapies for peripheral nerve repair is the term “minimal manipulation.” This is defined as “processing that does not alter the biology of the cell” [120]; however, stem cell therapies often require multistage processing especially for nonhomologous use. From a tissue engineering perspective, the stem cells would often be differentiated in vitro prior to being combined with a scaffolding material, for example, collagen to form artificial tissue [99, 121], and therefore the tissue-engineered device would be classed as more than minimally manipulated. Unger et al. [122] reviewed the pivotal role of GMP with regard to hESCs lines; however, there are still challenges to develop a standard operating procedure for their derivation. Reviews by Bieback et al. [123] and more recently Sharma et al. review clinical scale manufacturing and translation of mesenchymal stromal cells with a focus on regulatory frameworks and GMP.

Several authors also comment on the lack of regulatory harmonisation where subtle differences in GMP protocols can prevent a certain therapy moving forward [124–126]. For example, these differences have been noticed in sterilising procedures, control of starting materials, and disparities in definitions of quality, safety, and efficacy. The International Society for Stem Cell Research (ISSCR) set out guidelines describing how stem cell therapies can be responsibly translated [127]. Abiding by these international guidelines also offers a certain degree of standardisation since all stem cells will be manufactured in a reproducible manner to meet present specifications that ensure efficacy and safety.

4.4. Stem Cell Extraction and Isolation

Stem cells can be obtained from various sources, with each technique presenting different challenges. In light of this, the European commission has issued directives to ensure cross-border harmonisaton in stem cell donation, procurement, processing and preservation [128]. Here, some of the differences in obtaining stem cells from various sources will be briefly discussed.

In the UK, the Human Fertilisation and Embryology Authority (HFEA) is an independent regulator responsible for the procurement of gametes and the associated processing involved in the creation of an embryo and this includes overseeing the derivation of embryonic stem cell lines [129]. Once the inner cell mass is disassociated from the embryo, the originator is obliged to donate samples to the United Kingdom Stem Cell Bank (UKSCB) and the stem cell line is regulated by the Human Tissue Authority [130]. Isolation of mesenchymal stem cells can involve multistage ex vivo processing and numerous protocols are available [131–135].

Umbilical cord blood is commonly collected by inserting a cannula into an umbilical vein and allowing the blood to drain out; this is often known as gravity-assisted collection [136]. More recent attention is beginning to focus on other neonatal tissues that can be clinically translated, for example, Wharton’s jelly of the umbilical cord, amniotic membrane, and placenta [137–139].

The most widely used method of extracting bone marrow is through a bone marrow biopsy commonly from the posterior superior iliac spine or crest usually under general anesthetic [140, 141]. The BMSCs reside in the bone marrow stroma in small quantities [142] and this number decreases with age; hence, using this as an autologous source of stem cells to treat an elderly population would be challenging [143]. The abundance and accessibility of adipose tissue make the ADSCs a potentially more attractive mesenchymal stem cell source [144]. Large quantities of subcutaneous adipose tissue can be obtained through minimally invasive liposuction surgery usually under local anesthetic with minimal donor site morbidity.

Dental pulp stem cells can be isolated from discarded wisdom or deciduous teeth therefore bypassing the need for invasive tissue harvest associated with other stem cell sources [145]. Teeth contain various different populations of stem cells that can be isolated in different ways and stored in stem cell banks. Martens and colleagues [146] have reviewed dental stem cells and their potential role in neural regeneration.

While autologous adult neural stem cells can be harvested and may be useful for peripheral nerve regeneration, their extraction requires intricate surgery from either the dentate gyrus of the hippocampus or the subventricular zone of the lateral walls of the lateral ventricles of the brain [147]. The invasiveness of the procedure together with the fact that they are present in low numbers may limit their clinical applications [148]. Compared to adult NSCs, embryonic and foetal NSCs are relatively easily cultured and grown [149], and the majority of NSC lines available today are of foetal origin [150].

Other stem cell sources being investigated for use in peripheral nerve tissue engineering include the hair follicle stem cells and skin derived stem cells [67, 71]. The use of hair follicle stem cells in particular for nerve regeneration can potentially overcome problems associated with other stem cell sources as they can be easily harvested and are not associated with so many ethical issues [151].

4.5. Stem Cell Expansion

The addition of additives such as growth factors can differentiate a stem cell towards a particular lineage [152] although the large-scale amplification of stem cells also increases the mutation rate that could directly impact treatment with these cells [152, 153]. Recent work has also shown that long-term culture can alter the genetic composition of the cells [154, 155].

Currently, there is no optimal basal medium used for stem cell expansion. Some studies use Iscove’s Modified Dulbecco’s Media [36, 38], whereas others use Dulbeccos Modified Eagle’s Media [52, 156] or alpha-minimum essential medium [157]. Serum appears to be a key component for the expansion of some cells; hence, many media are supplemented with GMP grade Foetal Bovine Serum (FBS) to produce a formulated cocktail of proteins, growth factors, and nutrients. FBS is widely used throughout research and clinical studies although its commercial use is undesirable due to several inherent problems outlined in [158]. These include, but are not limited to, cross-species contamination, high content of xenogeneic proteins, and high batch-to-batch variation which all increase the regulatory burden. Nevertheless, the FDA has approved the use of GMP clinical grade FBS; however, [159, 160] show that immunogenicity against FBS proteins reduces the therapeutic benefit. With a focus on clinical translation, recent approaches have begun to explore defined serum-free and nonxenogeneic media options for multiple cell lineages [161–163]. Various bioprocessing approaches have been developed to support the large-scale expansion of therapeutic cells, including multilayer cell factories and closed-system automated bioreactors in accordance with GMP guidelines; these are detailed in [164].

4.6. Variability in Stem Cells

Recent literature describes the importance of donor age and time in culture in determining mesenchymal stem cell efficacy and quantity [165–167]. For example, a study by Siegel et al. [168] isolated BMSCs from 53 donors, aged between 13 and 80 years, and found that age and gender affect expression of certain makers and consequently BMSC function. A study by Choudhery et al. [169] recently described the negative effect of age on ADSCs whereby aged MSCs displayed senescent features, reduced viability, and proliferation and differentiation potential when compared to ADSCs from young donors. Conversely, a study by Choi et al. [170] used tonsil-derived mesenchymal stem cells and suggested that donor age and long-term passage had little effect.

Emerging studies have begun to understand the limitations of in vitro stem cell assays since it is becoming increasingly apparent that in vitro data do not correlate with in vivo results [171, 172].

There are also differences in the proliferation capacity of stem cells; for example, to generate a culture that is confluent in approximately 5–7 days, it is common to seed freshly isolated bone marrow stem cells in the range of 20,000–400,000 cells/cm² whereas ADSCs only require to be seeded at a density of 3500 cells/cm² to achieve the same level of confluence in the same time [144]. Considering this, Fossett and Khan [173] have recently discussed methods to optimise hMSC numbers for clinical application. A short communication by Zhou et al. [174] describes that seeding density of mouse embryonic stem cells and also quality of embryonic bodies directly effect the neural differentiation of the cells.

4.7. Preservation

Following isolation of the desired stem cells they can be either directly used for therapy or stored frozen. The cryopreservation of stem cells including induced pluripotent stem cells with consideration of GMP is reviewed by Hunt [175]. Currently, the gold standard method for cryopreservation involves suspending embryonic or mesenchymal stem cells in a mixture of FBS, growth media, and usually 10% dimethylsulfoxide (DMSO). This solution undergoes a slow-freeze protocol; however, thawing is rapid. Interestingly, this protocol is effective for murine and embryonic stem cells; however, storing human embryonic stem cells under these conditions is plagued with poor cell survival [176]. Various cryopreservation protocols for embryonic stem cells have been reviewed by [177, 178]. Different research groups are optimising preservation protocols with novel techniques to ensure maximal cell viability after thaw [179, 180]. Similarly, numerous studies investigated the effects of cryopreservation conditions on MSCs and demonstrated that they can be stored without loss of function [181]. In fact, a study by Ginis et al. [182] showed that BMSCs can be successfully preserved for the long term and delivered to the clinic in protective hypothermic storage in the short term. There are concerns about the toxicity of DMSO in humans; thus, there is substantial interest in reducing or completely removing DMSO from the preservation solution [183, 184].

5. Conclusion

PNI continues to be an area of unmet clinical need and advances in tissue engineering would be a welcome therapeutic option. To this end, a number of studies have highlighted the ability of stem cells from a variety of sources to differentiate into Schwann cells as starting material for these constructs. This competitive environment is both healthy and beneficial; each different type of stem cell will have its own unique set of advantages and disadvantages and success may ultimately lie in selecting the correct source for the desired tissue engineering strategy. Although there is currently no licensed stem cell based product for PNI, it is important that we take these issues into account at an early stage in development. It is highly encouraging that there is a clear international effort to develop and characterize stem cells for Schwann cell based engineered tissue for therapeutic application within the PNI field.

Competing Interests

The authors declare that there is no conflict of interests regarding the publication of this paper.

Authors’ Contributions

Kulraj Singh Bhangra and Francesca Busuttil contributed equally to this paper.

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