Chitosan tubes enriched with fresh skeletal muscle fibers for delayed repair of peripheral nerve defects

Abstract

Nerve regeneration after delayed nerve repair is often unsuccessful. Indeed, the expression of genes associated with regeneration, including neurotrophic and gliotrophic factors, is drastically reduced in the distal stump of chronically transected nerves; moreover, Schwann cells undergo atrophy, losing their ability to sustain regeneration. In the present study, to provide a three-dimensional environment and trophic factors supporting Schwann cell activity and axon re-growth, we combined the use of an effective conduit (a chitosan tube) with a promising intraluminal structure (fresh longitudinal skeletal muscle fibers). This enriched conduit was used to repair a 10-mm rat median nerve gap after 3-month delay and functional and morphometrical analyses were performed 4 months after nerve reconstruction. Our data show that the enriched chitosan conduit is as effective as the hollow chitosan conduit in promoting nerve regeneration, and its efficacy is not statistically different from the autograft, considered the “gold standard” technique for nerve reconstruction. Since hollow tubes not always lead to good results after long defects (> 20 mm), we believe that the conduit enriched with fresh muscle fibers could be a promising strategy to repair longer gaps, as muscle fibers create a favorable three-dimensional environment and release trophic factors. All procedures were approved by the Bioethical Committee of the University of Torino and by the Italian Ministry of Health (approval number: 864/2016/PR) on September 14, 2016.

Introduction

Peripheral nerve regeneration is affected by different factors, including the time span occurring between the injury and the repair (Sunderland, 1990; Hoke, 2006). Indeed, in polytraumatic patients nerve reconstruction might be delayed in time up to several weeks to allow the resolution of concomitant more severe injuries (Evriviades et al., 2011; Moore et al., 2015).

The consequence of a secondary surgery is the progressive degeneration of the distal nerve stump that leads to target organ (skeletal muscle and sense organs) denervation with a final unsatisfactory functional recovery, also after a successful microsurgical nerve repair (Sulaiman and Gordon, 2013). This poor clinical outcome can eventually result in life-long paralysis with motor and sensory deficits that compromise patients’ quality of life.

Currently, the gold standard technique used to bridge large peripheral nerve defects is the autologous nerve graft (autograft). However, this procedure has some limitations including additional surgery need, donor side morbidity and limited donor nerve availability (Hallgren et al., 2013; Faroni et al., 2015). These limitations inspired researchers to develop alternative techniques to repair large nerve defects.

In the last years, artificial peripheral nerve guidance conduits made by non-nervous materials, either of biological or synthetic origin, have been widely investigated. Among these, muscle-in-vein combined conduits have been employed as alternative to autograft for injured nerve repair, leading to good functional regeneration (Battiston et al., 2000a, b; Marcoccio and Vigasio, 2010; Manoli et al., 2014). The combination of a structure that prevents muscle fiber dispersion (the vein) with a structure that forestalls vein collapse and creates a favorable environment for Schwann cell migration and axonal regrowth (the muscular tissue) is the basis of this technique success (Raimondo et al., 2005).

In recent studies, a chitosan nerve guidance conduit gave promising preclinical results in both standard and critical length nerve reconstruction (Haastert-Talini et al., 2013; Meyer et al., 2016; Bak et al., 2017; Stenberg et al., 2017) and is now available for peripheral nerve gap reconstruction in human patients (Reaxon® Nerve Guides; Medovent GmbH, Germany).

We recently evaluated peripheral nerve regeneration after primary nerve reconstruction using a chitosan nerve conduit filled with fresh skeletal muscle fibers (muscle-in-tube, MIT). We demonstrated that, although MIT performance 12 weeks after surgery was comparable to hollow chitosan conduit in terms of functional recovery and quantitative morphometry, in vitro experiments and in vivo short-term analyses demonstrated that fresh skeletal muscle can be a source of important gliotrophic factors, absent in the hollow tube (Ronchi et al., 2018).

The aim of this study was to evaluate whether MIT can support nerve regeneration after a delayed surgical peripheral nerve reconstruction (“secondary repair”).

Materials and Methods

Animals and surgery

Fifteen female adult Wistar rats were used (ENVIGO, Bresso, Italy; body weight 200–250 g, approximately 2 months old). Animals were housed in a room with controlled temperature and humidity, with light/dark cycles of 12/12 hours, fed ad libitum with food and water.

Every attempt was made to reduce animal suffering. All procedures were approved by the Bioethical Committee of the University of Torino and by the Italian Ministry of Health (approval number: 864/2016/PR) on September 14, 2016. Moreover, these procedures are in agreement with the National Institutes of Health guidelines (NIH Publication No. 85-23, revised 1996), the Italian Law for Care and Use of Experimental Animals (DL26/14), and the European Communities Council Directive (2010/63/EU).

During surgical procedures, animals were placed under general anesthesia induced by intramuscular injection of Tiletamine and Zolazepam (Zoletil, Carros, France; 3 mg/kg) and were located in supine position.

Using an incision from the nipple to the elbow crease, the left median nerve was exposed, isolated and transected about in the middle of the exposed part; the proximal nerve stump was buried in the pectoral muscle to prevent regeneration; the distal stump was blocked through stitches to adjacent innervated muscles and allowed to degenerate for 3 months.

Three months after median nerve denervation, median nerves were repaired according to the following experimental groups [Figure 1]:{Figure 1}

- Chitosan-based hollow tube: an 8 mm nerve segment was removed and a 10-mm long chitosan tube was used to bridge the nerve defect by inserting 1 mm of the two nerve ends inside the conduit. The nerve guide was sutured at each end.

- Chitosan-based tube filled with fresh skeletal muscle –MIT: an 8 mm nerve segment was removed and a 10-mm long chitosan tube enriched with a longitudinal piece of the pectoralis major muscle (withdrawn from the same animal) was used to bridge the nerve defect by inserting 1 mm of the two nerve ends inside the conduit.

Medical grade chitosan for chitosan nerve guides manufacturing was supplied by Altakitin SA (Lisbon, Portugal). Chitosan-based tubes (Reaxon® Nerve Guide) were supplied by Medovent GmbH (Mainz, Germany).

- Autograft: an 10 mm median nerve segment was cut out, reversed (distal-proximal) and sutured to the nerve ends of the same animal.

To prevent interferences during the grasping test, the right median nerve of each animal was transected at the middle third of the brachium and its proximal stump was sutured to the pectoralis major muscle to avoid spontaneous reinnervation.

All animals were sacrificed after 4 months from the surgery by an overdose of Tiletamine and Zolazepam (40 mg/kg; Zoletil) and a segment of 5 mm of the regenerated distal nerve stump was harvested and analyzed for stereological and morphometrical analysis.

Grasping test

The strength of the flexor digitorum profundus muscle and flexor digitorum sublimis muscle, which are both innervated by the median nerve in rats, was assessed by the grasping test. The grasping test was therefore performed to estimate functional recovery after nerve reconstruction. The analysis was carried out before animal sacrifice (4 months after nerve repair) following the same procedure previously described (Papalia et al., 2003; Ronchi et al., 2009). Rats were acclimatized before the testing. Each animal was tested three times and the average value was recorded.

High resolution light microscopy and electron microscopy analysis

Regenerated median nerve distal portions, harvested 4 months after repair, were processed for resin embedding as previously described and semi-thin sections (2.5 µm thick) were cut and stained with 1% toluidine blue for light microscopy analysis (Ronchi et al., 2017). Ultra-thin sections (70 nm thick) were cut with the same ultramicrotome used for semi-thin sections. Sections were analyzed using a JEM-1010 transmission electron microscope (JEOL, Tokyo, Japan) equipped with a Mega-View-III digital camera and a Soft-Imaging-System (SIS, Münster, Germany) for image acquisition.

Morphometrical analysis

The quantification of myelinated nerve fibers was performed on the toluidine blue-stained semi-thin sections. A systematic random sampling protocol earlier described was performed (Geuna, 2000; Geuna et al., 2000) with a magnification of 100×. In each sampling field, a 2-D dissector procedure was carried out. Total number of myelinated fibers, fiber and axon diameter, myelin thickness, g-ratio and fiber distribution were then estimated. IM50 image manager system (Leica Microsystems) was used for these analysis.

Statistical analysis

For statistical analysis IBM SPSS Statistics 25.0 software (IBM, Armonk, NY, USA) was used. Data were expressed as the mean + standard deviation (SD). Data sets were processed by one-way analysis of variance (ANOVA) with Bonferroni correction.

Results

To evaluate the efficacy of chitosan tubes enriched with fresh skeletal muscle fibers (MIT) in promoting regeneration after delayed nerve repair, median nerves were repaired 3 months after injury and regenerated nerves were analyzed 4 months after repair. Three experimental groups were analyzed: autograft (positive control), hollow chitosan tube (not enriched control), MIT. Macroscopic images of the regenerated nerves can be appreciated in [Figure 2]. Inside the hollow tube [Figure 2]B, the regenerated nerve segment is clearly visible (it is notable that it is thinner than proximal and distal nerve stumps); MIT conduit is still full of muscle tissue that has not degenerated yet, therefore the regenerated fibers are not visible [Figure 2]C.{Figure 2}

Morphological evaluation

Morphological evaluation carried out on toluidine blue-stained semi-thin sections obtained distally to the graft reveals that regenerated nerves in the three experimental groups exhibit many regrowing myelinated fibers organized in microfascicles [Figure 3]A, [Figure 3]E, and [Figure 3]I. Electron microscopy images allow better appreciating the ultrastructure of myelinated fibers with well-defined axoplasm and well-organized myelin sheaths; moreover, unmyelinated fibers can also be detected [Figure 3]B, [Figure 3]C, [Figure 3]D, [Figure 3]F, [Figure 3]G, [Figure 3]H, and [Figure 3]J, [Figure 3]K, [Figure 3]L.{Figure 3}

Functional recovery analysis

[Figure 4]A reports the results of the functional recovery 4 months after nerve repair. The function of finger flexor muscles, innervated by the median nerve, was recovered in the three experimental groups with no significant differences among them.{Figure 4}

Morphometrical analysis

Quantitative analysis on semi-thin sections shows that the total number of myelinated fibers, obtained with stereological methods, is not statistically different among groups (autograft group has the highest number of myelinated fibers, as expected, but this value is not statistically different compared to both the hollow chitosan and the MIT groups) [Figure 4]B.

Regarding size parameters (axon and fiber size, myelin thickness and g-ratio) [Figure 4]C and [Figure 4]D, no significant differences can be appreciated among groups.

The analysis of individual fiber g-ratio/axon diameter correlation [Figure 4]E, [Figure 4]F, [Figure 4]G shows that the MIT group displays a regression line with a lower slope compared with the other two groups (autograft and hollow chitosan groups have overlapping regression lines).

Finally, fiber diameter frequency distribution shows that the three experimental groups exhibited a fiber diameter unimodal distribution. In particular, all these groups show a peak at 2–2.5 µm [Figure 4]H, but the MIT group has a higher percentage of bigger fibers (> 4 µm diameter) compared with the other two groups [Figure 4]I.

Discussion

Traumatic lesions of peripheral nerves are of clinical importance owing to their high incidence, resulting as a consequence of motorcycle or car accidents, domestic falls, work accidents or after surgeries (iatrogenic nerve injuries) (Jones et al., 2016). The peripheral nerve regenerative ability has been recognized for more than a century; however, clinical and experimental evidences show that such regeneration is often unsatisfactory, especially following severe lesions: approximately 50% of surgical cases achieves normal to good function (Pfister et al., 2011).

Although primary repair (within 1 week) is the optimal approach for peripheral nerve injuries, secondary (delayed) repair is indicated when an immediate repair is not possible due to other concomitant and complicating injuries (Griffin et al., 2014) and, unfortunately, the longer is the delay, the worsen is the prognosis. Indeed, nerve regeneration after delayed nerve repair is often incomplete, due to many factors, including the inability of the target organ to recover from atrophy, the inability of injured axons to completely regenerate and the inability of Schwann cells to sustain regeneration (Grinsell and Keating, 2014).

After injury, chronically denervated distal nerve stump undergoes several changes, both morphological and molecular. From a molecular point of view, the regeneration-associated genes (α1-tubulin, actin and growth associated protein 43), the ciliary neurotrophic factor, the transcription factor c‐Jun, Neuregulin1, S100 and glial fibrillary acidic protein are drastically reduced (Sendtner et al., 1992; Gordon and Tetzlaff, 2015; Jessen and Mirsky, 2016; Ronchi et al., 2017). On the contrary, the neurotrophic factors brain-derived neurotrophic factor, glial cell-derived neurotrophic factor and the p75 receptor are up-regulated (Michalski et al., 2008; Ronchi et al., 2017). Moreover, after long-term denervation Schwann cells undergo atrophy, and endoneurial tubes (the basal laminae of Schwann cells) progressively shrink and decrease in diameter (Hoke, 2011).

Several studies aimed to find new strategies to improve nerve regeneration after delayed nerve repair. Recently, chitosan conduits (regular or corrugated, hollow or filled with a longitudinal z-folded chitosan film) were used to bridge a 15-mm nerve gap after a 45-day delayed repair (Stenberg et al., 2017; Stößel et al., 2018), demonstrating their efficacy, although less effective in comparison to immediate repair (Meyer et al., 2016).

In the present study, the chitosan conduit was enriched with fresh muscle fibers (MIT) because it has been shown in vitro and in vivo that muscle cells produce and release gliotrophic factors important to support axon re-growth and Schwann cell activity (Montoya et al., 2009; Ronchi et al., 2018).

In a previous study we demonstrated that MIT efficiently supports peripheral nerve regeneration when used for a primary repair (Ronchi et al., 2018); therefore, the aim of this study was to evaluate the efficacy of this enriched conduit to reconstruct a 10-mm nerve gap after 3 months of denervation.

This study results show that MIT is as effective as hollow chitosan conduit in promoting nerve regeneration after delayed 10-mm nerve gap reconstruction. Indeed, functional and quantitative morphological data do not show statistic differences between these two experimental groups and autograft, which is the “gold standard” technique for nerve reconstruction (autograft shows more regenerated fibers and better performance in functional test, but these values are not statistically significant compared to both MIT and hollow chitosan conduit).

Therefore, data about hollow chitosan conduit confirm the results obtained in other previous studies (Stenberg et al., 2017; Stößel et al., 2018), while enrichment with fresh nerve fibers does not seem to further improve its effectiveness; nevertheless, a slightly higher percentage of myelinated nerve fibers with a diameter bigger than 4 µm can be observed.

The reasons for the positive results obtained with MIT –but not better than those obtained with hollow chitosan tube –may be different: (i) the release of factors by fresh muscle fibers occurs within the first few days; probably the muscle has a short-time beneficial effect that is lost over time and after 4 months is no longer perceptible; (ii) the hollow conduit, as previously extensively demonstrated (Haastert-Talini et al., 2013; Gonzalez-Perez et al., 2015; Meyer et al., 2016; Shapira et al., 2016; Bak et al., 2017), is very effective in promoting nerve regeneration; for this reason, the different strategies to further enrich it, to date, did not further improve its effectiveness, especially for short nerve gaps: the use of fresh muscle fibers as a filler could probably give better results when used to repair larger gaps (> 20 mm). Indeed, hollow tubes not always lead to good results after long defects and conduit enrichment might create a favorable environment for nerve re-growth. In particular, muscle fibers create a favorable three-dimensional environment provided by their basal lamina useful for Schwann cell migration and axonal regrowth.[35]

Author contributions: Study conception and design: SG, BB, PT; data collection and processing: AC, BEF, GG, SR, GR; data analysis, statistical analysis, and interpretation: AC, BEF, GG, SR, GR; preparation of the figures: BEF, GR; manuscript drafting: GG, BEF, GR; manuscript revising and editing: SG, BB, PT. all authors approved the final version of the manuscript.

Conflicts of interest: The authors report no conflicts of interest.

Financial support: This study was supported by the European Community’s Seventh Framework Programme (FP7-HEALTH-2011), No. 278612 (to SG); and by Compagnia di San Paolo, No. D86D15000100005; InTheCure project (to SR). The funding bodies played no role in the study design, in the collection, analysis and interpretation of data, in the writing of the paper, and in the decision to submit the paper for publication.

Institutional review board statement: All procedures were approved by the Bioethical Committee of the University of Torino and by the Italian Ministry of Health (approval number: 864/2016/PR) on September 14, 2016. Moreover, these procedures are in agreement with the National Institutes of Health guidelines (NIH Publication No. 85-23, revised 1996), the Italian Law for Care and Use of Experimental Animals (DL26/14), and the European Communities Council Directive (2010/63/EU).

Data sharing statement: Datasets analyzed during the current study are available from the corresponding author on reasonable request.

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Peer review: Externally peer reviewed.

Funding: This study was supported by the European Community’s Seventh Framework Programme (FP7-HEALTH-2011), No. 278612 (to SG); and by Compagnia di San Paolo, No. D86D15000100005; InTheCure project (to SR).