Добавил:
kiopkiopkiop18@yandex.ru t.me/Prokururor I Вовсе не секретарь, но почту проверяю Опубликованный материал нарушает ваши авторские права? Сообщите нам.
Вуз: Предмет: Файл:

Ординатура / Хирургия / Библиотека им академика М.И. Перельмана / Книга_896_Библиотеки_им_академика_М_И_Перельмана

.pdf
Скачиваний:
0
Добавлен:
31.08.2026
Размер:
33 Мб
Скачать
ab
cd
(msec)
8 Regeneration oftheSkin andPeripheral Nerves intheAdult
https://t.me/med1917
11
10
9
8
7 6
(mV)
5
4 3 2
1
0
Normal Nerve
A fiber Peak
Regenarated Nerve
A-fiber Peak
Regenarated Nerve
B-fiber Peak
Stimulas
0123 45
141
Fig. 8.4 Evidence of induced regeneration of the peripheral nerve using collagen-based nerve regeneration template. Histological micro­graphs of nerve tissue postxed with osmium tetroxide and stained with toluidine blue. The magnication for each micrograph is the same; scale bars, 10μm. (a) Tissue regenerated through the midportion of a matrix-lled large-pore collagen (LC/M) implant at 30weeks. Note the large number of axons in this cross-section with the majority of axons being small in diameter. The largest axons have diameters of approxi­mately 7μm. Many Schwann cells are visible with some actively par­ticipating in myelination. The blood vessel that is visible in this micrograph was characteristic of the caliber of most vessels present in the regenerated tissue. (b) Tissue regenerated through the midportion of a LC/M implant at 60 weeks. Compared to 30 weeks, the axons are much larger (diameters up to 12μm) and have thicker myelin sheaths. Also, fewer small diameter axons are visible. Few nonmyelinating Schwann cells are visible at 60weeks. (c) Normal nerve tissue from the level of the lesion is shown as a control. Note the number of large diam­eter bers and the thickness of the myelin sheaths compared to the
Limitations ofCollagen-Based Scaolds asRegenerative Devices
As stated earlier, these clinically approved devices do not induce regeneration of entirely normal organs. For example, skin regenerated by the use of collagen-based scaffolds may lack several appendages (i.e., sweat glands, hair follicles), although there have been increased improvements with such outcomes [56]. Future work may focus on speeding the rate of cell migration and angiogenesis within the device (angio-
regenerated nerves. (d) Typical oscilloscope tracings of A-ber and B-ber compound nerve action potentials for normal sciatic nerve and nerve regenerated through a LC/M implant at 60weeks postimplanta­tion. The A-ber peak for the regenerated nerve has a signicantly smaller amplitude than the normal nerve control. This was typical of all regenerated groups. In contrast, the conduction velocity of the regener­ated nerve, although signicantly slower than normal, was approaching normal values. The latency is measured along the x-axis from the stimu­lus to the peak and then combined with the constant distance between electrodes to determine conduction velocity. The dashed line indicating the B-ber peak has been added on to the tracing for reference. Note that the normal nerve tracing has no visible B-ber peak. In the regener­ated nerves, the B-ber peak was similar and visible in all groups. (Reproduced from Chamberlain LJ, Yannas IV, Hsu HP, and Spector M. Collagen-GAG Substrate Enhances the Quality of Nerve Regeneration through Collagen Tubes up to Level of Autograft. Exp Neurol 1998: 154: 315–329)
genesis peaks in 7–14days in a murine model) with the goal of improving regeneration, increasing the safety prole of the device, and decreasing the risk of infection. Peripheral nerves that regenerated with tubular collagen-based scaf­folds exhibit conduction velocity proles that are somewhat slower and weaker than with normal nerves (although scaf­folds that have been recently synthesized, but are not com­mercially available, improve signicantly on the clinically available device).
142
CSR++ = 100
https://t.me/med1917
Table 8.3 Summary of FDA-approved regeneration devices
Device name Approval year Indications Clinical results
Skin
Integra Dermal Regeneration Template® (DRT)
PolyNovo Novosorb Biodegradable Temporizing Matrix (BTM)
Peripheral Nerve Neuragen
Polyganic’s Neurolac 2005 Severe peripheral nerve
GEM’s Neurotube 1999 Severe peripheral nerve
®
1996 and 2002 Severe burns,
reconstructive surgery, skin ulcers
2015 Second-degree burns,
acute/chronic wounds
2001 Severe peripheral nerve
injury
injury
injury
• 440 clinical cases cited
• 86.7% healing rate in diabetic patients with foot wounds [12]
• Viable option for stable closure of wounds in low-risk patients [15]
• Synthetic, biocompatible, biodegradable
• Less prone to infection and aggressive wound contraction compared to DRT [62]
• Successful use in various clinical settings
• Signicantly lower postoperative pain scores than control group [69]
• Sensory and motor function performance equal to direct repair group [69]
• Issues with biocompatibility, swelling, degradation rate, rigidity, patient complaints, and automutilation [77]
• More mixed results due to slower rate of recovery, sensory changes, and uncommon complications
A. Z. Yang et al.
The Defect Closure Rule
Careful review of the literature suggests that no more than three distinct processes are used to close an anatomically well-dened defect (dermis-free defect) in skin wounds: contraction originating from the edges of the defect, scar for­mation by stromal broblasts (followed by epithelialization of scar), and regeneration.
Kinetic data extending continuously over lengthy periods are rarely available from regeneration experiments and often difcult to compare from one study to another. One approach to studying the regenerative activity of exogenous agents on the healing process is to establish two standardized congura­tion states (e.g., initial and nal state) and to evaluate the total change that is caused during this xed period in the healing process. In the absence of kinetic data, the defect closure rule bridges the gap by presenting a quantitative description of the healing process through comparison of snapshots of the ini­tial and nal stages of wound healing. The initial state of con­guration is the anatomical description of the recently generated defect, characterized by the loss of structural conti­nuity in one or more tissues, beginning of exudate ow, and loss of physiological homeostatic control of the organ. As defect healing progresses, the original area, A0, eventually diminishes spontaneously due to one or more of the three pro­cesses mentioned. The area of the closed defect (the closed wound) comprises tissues that result either from contraction (%C), scar formation (%S), or regeneration (%R), and the conguration of the nal state can be described by the follow­ing simple relation, called the defect closure rule:
Equation 8.1 states that the defect closure in any organ can be described by only three outcomes: contraction, scar
(8.1)
formation (neuroma or brosis), and regeneration (partial or total). For the idealized case of early fetal wound healing (spontaneous regeneration), contraction and scarring are absent (C, S = 0) and R = 100 (regeneration). For normal defect closure in adult mammals following irreversible injury (repair), regeneration is absent (R = 0) and C + S = 100 (repair).
The literature describes several assays, such as simple measurements, histopathologic grading, biochemical testing, and image analysis, that can be used to determine the con­guration of the nal state (recently closed defect) [80]. Functional assays especially can be used to qualitatively identify the physiological nature of the tissue and assist in providing a quantitative measure of its incidence in the nal state in terms of the numerical values of these three quanti­ties (C, S, R). The defect closure rule may be interpreted as a conservation principle: provided that the magnitude of two individual terms have been determined, the magnitude of the remaining process may be calculated. Defect closure data is expressed using the following convention: [%C, %S, %R].
The defect closure rule is useful in evaluating the activity of unknown reactants as inductive agents of regeneration. This quantitative description of the structure and function of the injured organ at its nal state has shed interesting light on the relationship between the characteristic elements of the adult healing response (contraction or scar synthesis, or both) and regeneration.
Prevalence ofContraction During Spontaneous Healing
In the skin, the defect closure rule has been used to present data on the conguration of the nal state following sponta­neous healing of the anatomically well-dened defect (dermis- free defect) in several species. In all cases of sponta-
[]
()
[]
+
()
8 Regeneration oftheSkin andPeripheral Nerves intheAdult
https://t.me/med1917
143
neous healing of full-thickness skin wounds, it was ensured that the contribution of regeneration to defect closure was negligible (R=0). Skin contraction was measured directly as the reduction in initial wound surface area by inward (cen­tripetal) movement of the skin from the margins of the wound. Scar formation was frequently studied qualitatively by histology. In a few cases, scar formation was conrmed quantitatively by the use of laser light scattering, which was used to measure the average degree of collagen ber orienta­tion and thereby deduce on the identity of the tissue present in the healed injury site [81]. More recently, various advanced imaging techniques, such as optical coherence tomography and confocal microscopy, have allowed greater visibility of the scar microstructure, allowing for both qualitative obser­vations and quantitative spatial pattern analysis [8284]. Values for the percentage of initial defect area closed by epi­thelialized scar (S) were determined using the simplied defect closure rule for repair (S=100– C).
The contribution of the various methods of defect closure in anatomically well-dened defects is species-dependent. In rodents, where the integument is mobile, contraction is by far the main engine of closure of skin wounds, while scar formation has been shown to be quantitatively much less important. The spontaneous healing of a full-thickness skin wound in the guinea pig is characteristic of several rodents and lagomorphs (rabbits) and results in the following nal state conguration: [91, 9, 0] [85, 86]. In general, C>>S and defect closure for adult rodents and rabbits reduces to C100. Alternatively, the approximation of the nal state in rodents is expressed as [100, 0 0]. In humans, where the integument is tethered more securely onto subcutaneous tis­sues, contraction and scar formation contribute approxi­mately equally to wound closure. Experimentally, the spontaneous healing of full-thickness skin defects in the human (R=0) results in a nal state represented by [37, 63, 0] [87].
In the absence of direct quantitative observations, histo­logical analysis was used to describe the closure of the fully transected peripheral nerve in the adult rat. Spontaneous healing results in the reduction of the initial area of cross­sections of nerve trunks by 95% with neuroma formation (neural scar) accounting for the remaining 5%. The resulting estimation of the nal state conguration was [95, 5, 0] [88,
89].
The contraction of a wide array of organs in response to trauma is well documented in both animals and humans, yet these reports are almost exclusively of a qualitative nature [9094]. With very few exceptions, the sole organ in which contraction has been studied systematically to date is the skin. Despite the dearth of widespread quantitative data, the prevalence of contraction must not be overlooked; it appears to be a critical outcome of the spontaneous healing response throughout the adult organism.
The Antagonistic Relation Between Contraction andRegeneration
The characteristic elements of the adult healing response (contraction or scar synthesis, or both) must be controlled in order for induced regeneration to occur. Extensive data, including empirical data on the nal state of the defect in response to various reactants, suggest that during healing of a severe injury, contraction antagonizes regeneration [1].
Induced regeneration of the skin, peripheral nerve trunks, and the conjunctival stroma was accompanied in each case by direct observation of a signicant reduction in contraction as a mode of defect closure. Conjunctival and peripheral nerve regeneration studies were guided by earlier studies of skin regeneration. The partial skin was rst induced to regen­erate in the adult guinea pig. The spontaneous healing behav­ior of the untreated dermis-free defect in this organism resulted in a nal conguration of [91, 9, 0]. Grafting an identical well-dened skin defect with a highly porous copo­lymer of type I collagen and chondroitin 6-sulfate (referred to as a dermis regeneration template, DRT) (Fig.8.5a) abol­ished scar synthesis and led to the regeneration of a small mass of dermis and subsequent synthesis of an overlying epi­dermis within the defect. In the context of the defect closure rule, the regenerative activity of the cell-free DRT on the conguration of the nal state [1] was as follows:
In addition, the DRT led to a signicant delay in wound contraction over 25days.
When a DRT seeded with keratinocytes (KC) was grafted into an identical defect, the result was much more pronounced:
KC-seeded DRTs accomplished rapid wound closure through the partial regeneration of the skin (simultaneous synthesis of a physiological dermis and epidermis, described earlier) and completely arrested contraction at 35–40 days [17].
The cell-free DRT that induces partial skin regeneration comprises the regenerative component of the two-layer device (Integra Dermal Regeneration Template (DRT)®) approved by the FDA for the restoration of a physiological epidermis and dermis in patients suffering from severe burns as well as those undergoing plastic and reconstructive sur­gery of the skin, as described in an early study [19] and reviewed recently [95].
Growth factors [96, 97], epidermal cell suspensions, and cell sheets [98] exhibited negligible regenerative activity when added to full-thickness skin wounds in other rodent models. These reactants did not signicantly alter the con­guration of the nal state or the extent of contraction delay. Similarly, a number of synthetic polymer scaffolds [99, 100]
92 80 89 011,, ,, DRT
91 90 28 072,, ,, DRTKC
144
ab
[]
()
[]
()
[]
()
[]
[]
+
()
 
 
 
 
https://t.me/med1917
A. Z. Yang et al.
Fig. 8.5 Induced regeneration of the dermis and peripheral nerve using scaffold composed of type I collagen and chondroitin 6-sulfate. (a, top) A scaffold that has induced regeneration of the dermis in animals and humans. Composition: graft copolymer of type I collagen and chon­droitin 6-sulfate. Scanning electron micrograph. Pore channel orienta­tion is almost completely random. Average pore diameter, 80 μm (courtesy of E.Soller, MIT). (b, bottom) Peripheral nerve was induced
failed to induce physiological dermis (or skin) regeneration. These observations focus attention on the mechanism of scaffold regenerative activity, to be discussed later.
Quantitative studies of induced regeneration of peripheral nerves were conducted in the adult rat. The spontaneous healing behavior of the untreated transected peripheral nerve in this organism resulted in a nal conguration of [95, 5, 0] that was estimated using histological analysis. Insertion of the fully transected nerve stumps into a silicone tube lled with a collagen-based tubular regeneration template (referred to as a nerve regeneration template or NRT) resulted in reduced contraction (as determined by histological analysis of cross-sectional areas of regenerates) and partial regenera­tion over a 10-mm-gap length [31, 32]. Contraction was abolished and the quality of regeneration improved signi­cantly when the NRT was used in conjunction with a degrad­able collagen tube. In the context of the defect closure rule, the regenerative activity of the NRT in each experimental conguration can be evaluated by inspecting the estimated characteristics of the nal state, as follows (the arrow indi­cates the change observed following use of the scaffold):
95 50 53 047,, ,, NRTinside silicone tube
95 50 00100,, ,, NRTinside collagen tube
The relative importance of each method of defect closure (C, S, and R) changes during animal development. A sharp change occurs during the fetal-adult transition in mammals (roughly during the third trimester of gestation), in which contraction replaces regeneration as the dominant method of
to regenerate across a 15-mm-gap (and eventually longer gaps) in the rat sciatic nerve using this scaffold as a bridge between the two stumps inside a silicone tube. In later studies the chemical composition of this scaffold was changed to GAG-free type I collagen. Pore channel orien­tation along the major nerve axis. Scanning electron micrograph. Average pore diameter, 20 μm [1]. Yannas I V. Tissue and Organ Regeneration in Adults. NewYork: Springer; 2001
closure [101103]. Similarly, as amphibian (frog) develop­ment progresses, contraction becomes a more prominent method of wound closure, as regeneration recedes and scar formation becomes more evident [58, 104, 105].
While scar has been widely considered the key barrier to regeneration in adults, quantitative study reveals that con­traction is the dominant mode of spontaneous closure in the skin and peripheral nerve defects. Studies of induced regen­eration in the skin, peripheral nerves using analogs of the extracellular matrix, indicate that scar formation is a process that is secondary to contraction: in studies of induced regen­eration in these organs, when contraction was even slightly inhibited, scar formation was totally abolished [1].
95 50 53 047,, ,,
95 50 00100,, ,,
Suppression of contraction in certain cases of impaired healing, e.g., following use of pharmacological agents, such as steroids was not accompanied by regeneration, indicating that suppression of contraction alone did not sufce to induce regeneration [1].
The available evidence supports the theory that selec­tively suppressed contraction in adult defects is required, but not sufcient to induce regeneration of the skin and periph-
92 80 89 011,, ,, DRT
91 90 28 072,, ,, skin,DRT KC
[]
[]
peripheral nerve,
NRTin silicone tube
peripheral nerve,
NRTin collagen tube
0
di
8 Regeneration oftheSkin andPeripheral Nerves intheAdult
https://t.me/med1917
145
eral nerves. This can be expressed in the context of the defect closure (Eq.8.1) rule as follows:
00
This condition describes an antagonistic relationship between contraction and regeneration in the closure of a defect. It suggests that successful induced regeneration strat­egies consist of reactants that block contraction without blocking other aspects of the healing process.
an
f
(8.2)
Repair: Mechanism ofContraction
Similarities in the mechanistic hypotheses for inducing regeneration of the skin and peripheral nerves originate in their common response to irreversible injury. Both organs spontaneously respond to injury by recruiting contractile cells that, if not properly suppressed, drive closure of the defect by contraction and scar synthesis rather than by regen­eration. Contraction of skin defects starts from a cell cluster at the edge of the defect and later extends across the entire defect area. In peripheral nerves, contraction primarily results from the activity of a circumferential sheath of con­tractile cells.
The Contractile Fibroblast Is theMain Cell Type Associated withContraction
The well-documented, macroscopic contraction that drives the closure of skin defects nds its origin at the cellular scale, arising from the individual contribution of contractile forces generated by differentiated myobroblasts [106113]. The current consensus is that myobroblasts (MFB) that are present in granulation tissue following skin wounding derive directly from broblasts and comprise an intermediate, con­tractile, cellular phenotype between the broblast and the smooth muscle cell. There is also evidence that undifferenti­ated broblasts may contribute to macroscopic contraction by applying traction to the ECM very soon after coming into contact with it [93, 109, 114118].
In response to external tension, broblasts exert sustained isometric force on their surrounding environment via a Rho/ Rho-kinase (ROCK)-mediated, actomyosin contractile appa­ratus [119121]. This three-dimensional, transcellular struc­ture consists of bundles of actin and non-muscle myosin microlaments called “stress bers.”
Of the many ultrastructural and biochemical factors that distinguish myobroblasts from their broblast precursors, the most useful operational distinction of MFB differentia­tion is the expression of the α-smooth muscle actin (α-SMA) phenotype [93, 114, 115]. Stress bers of immature myo­broblasts (called proto-myobroblasts) contain only beta­and gamma-cytoplasmic actins [93]. Additionally, differentiated myobroblasts exhibit stress bers typically arranged parallel to the long axis of the cell, nuclei which
consistently show multiple indentations or deep folds, and two cell-matrix adhesion macromolecules (vinculin and bronectin) [122, 123].
Simplistically, the myobroblast differentiation process can be described as a positive feedback loop that requires the concurrent action of at least three factors: the cytokine trans­forming growth factor-beta1 (TGF-β1), the presence of mechanical tension, and the ED-A splice variant of cellular bronectin (an extracellular matrix component) [115]. Fibroblasts respond to the development of mechanical ten­sion by upregulating TGF-β1 production and expressing the α-SMA isoform; in turn, α-SMA expression strengthens the contractile apparatus and increases tension development [115]. Recent work suggests that mature myobroblasts in skin granulation tissue link their cytoskeletons together using cadherin proteins, which allow them to generate even higher levels of force to drive wound closure [124].
Mechanism ofScaold Regenerative Activity
Structural Determinants ofScaold Regenerative Activity
Scaffolds that induce regeneration of the partial skin (Fig. 8.5a) possess a highly specic structure that is dis­tinctly different in pore structure and degradation rate from scaffolds that regenerate peripheral nerves (Fig.8.5b). The nature and duration of the contractile response as well as the structure of the two organs differ greatly as do the values for several of the structural parameters of the early scaffolds that were used to control contraction and induce regeneration in each organ. The scaffolds have a common ligand identity due to an identical chemical composition (type I collagen/gly­cosaminoglycan, 98/2 w/w ratio), yet they differ in average pore diameter (higher in the case of the DRT), the pore chan­nel orientation (axial for the nerve guide, random for the DRT), and degradation rate (a higher average molecular weight between cross-links, Mc [kDa] in the nerve guide leads to faster degradation) (Table8.4).
In skin wounds, the mechanism of induced regeneration has been elucidated through careful modulation of the DRT’s structural properties that impart contraction blocking activ­ity. DRTs that actively block contraction in skin wounds (and induce regeneration) have structural properties that accom­plish three main processes: (1) reduction in MFB number present in the wound, possibly due to inhibition of TGF-β synthesis, leading to downregulation of myobroblast recruitment; (2) blocking orientation of myobroblast axes in the plane of the defect where macroscopic contraction is observed; and (3) ensuring that DRT degradation time is suf­ciently long to ensure that contraction blocking persists for the duration of the interim myobroblast contractile response but not so long as to interfere with key regenerative processes.
146
https://t.me/med1917
A. Z. Yang et al.
Table 8.4
Structural parameter required for regenerative activity Skin regeneration
Type I collagen/GAG (w/w) residual collagen ber banding
Average molecular weight between cross-links (kDa)
Average pore diameter (μm) Pore channel orientation
GAG glycosaminoglycan Adapted from: Yannas IV, Tzeranis DS, Harley BA, So PT.Biologically active collagen-based scaffolds: advances in processing and characteriza­tion. Philos Trans A Math Phys Eng Sci. 2010 Apr 28;368(1917):2123–39
a
Approximate levels of structural determinants observed in skin regenerative studies conducted by grafting the scaffold on a full-thickness skin
wound [18]
b
Approximate levels of structural determinants observed in peripheral nerve regeneration studies performed by inserting the scaffold inside a nerve
conduit (the conduit connected the two stumps of the transected nerve across an experimental gap of dened length) [27, 28]
1. Apparent downregulation of TGF-β synthesis. The qua-
2. Blocking orientation of MFB axes in the plane of the
Structural determinants of regenerative activity of collagen/GAG scaffolds
a
98/2 approximately 5% of native collagen
5–15 40–60 Controls duration of undegraded
20–120 random 5–10 axial Ligand density
Nerve regeneration 98/2 approximately 5% of native
collagen
ternary structure of collagen bers is a requirement for the aggregation of platelets, an early component of the wound response. Platelet aggregation initiates a cascade of events that include the release of the cytokine TGF-β1, one of the main inductors of the myobroblast pheno­type. Collagen bers in the DRT maintain their tertiary (triple helical) structure but are practically free of band­ing (due to treatment with acetic acid during scaffold preparation). DRT apparently disrupts platelet aggrega­tion within the defect, reducing production of TGF-β1, and the recruitment of contractile myobroblasts to the wound site [125].
wound as well as MFB-MFB binding. Contraction of wound edges appears to require orientation of MFB axes in the plane of the wound as well as MFB-MFB binding and MFB-ECM binding. MFB binding on the extensive surface of the highly porous three-dimensional scaffold inhibits such orientation as well as inhibiting MFB-MFB and MFB-ECM binding. It is suggested that these mecha­nisms are additionally responsible for contraction block­ing by the scaffold. According to this suggested mechanism, contraction blocking requires extensive MFB binding onto a sufciently large scaffold surface, which must take place via specic integrin-ligand inter­actions. Fibroblasts bind onto a specic GFOGER ligand on a collagen surface via the α1β1 and α2β1 integrins [126]. When other structural properties are held constant, the ligand density of a scaffold increases with decreasing average pore size (since the specic surface area of the scaffold available for attachment is thereby increased). An appropriate ligand density appears to be necessary to disrupt extensive MFB-ECM binding responsible for the onset of macroscopic contraction in skin wounds.
When myobroblasts bind to specic DRT integrins that are distributed evenly in a three-dimensional, inter­connecting porous network, the axes of their contractile
b
Structural feature hypothetically responsible for contraction blocking
Ligand identity Reduction in recruitment of contractile cells
scaffold during contraction
Ligand orientation
apparatus become disoriented. At the cellular level, the randomized conguration of the preferential contractile axes that individual myobroblasts adopt in the presence of DRT leads to approximate cancellation of the macro­scopic mechanical forces that lead to two-dimensional contraction and scar synthesis in ungrafted skin wounds. When the pore diameter of DRT is increased much beyond the level of 120μm, the effective DRT ligand density drops to a value that does not provide sufcient binding of myobroblasts, and the contraction-blocking activity of the scaffold is lost [1, 127]. Similarly, a mini­mal average pore size exists that is necessary to ensure MFB migration inside the scaffold. According to this interpretation if the pore size is too small, MFB does not inltrate the scaffold, MFB-DRT ligand bonds do not form, and MFB contractile activity is not cancelled [18]. Experimentally, the highly planar orientation of myo­broblast axes that is characteristic of the spontaneous contractile response in ungrafted skin wounds is negligi­ble in the presence of DRT [128].
3. Duration of DRT in an undegraded state over the entire contraction process. It is known that the regenerative activity of the scaffold depends sensitively on its degrada­tion rate during skin regeneration [129] as well as during regeneration in the peripheral nervous system. To explain the data, it has been hypothesized that the DRT is required to undergo a process of isomorphous tissue replacement, in which the regenerate (dermis or nerve tissue) is synthe­sized at a rate which is of the same order as the rate of degradation of the DRT. The requirement for an optimal scaffold duration may reect the need to have the scaffold persist in an undegraded (insoluble) state over a period that matches the length of the contraction process in skin wounds and nerve wounds, thereby ensuring that the con­traction blocking activity is operative when it matters. In skin wounds the optimal half-life of degradation (tb) for DRT invivo is 14days, roughly matching the irreversible contraction response in ungrafted wounds (th) [17]. In
8 Regeneration oftheSkin andPeripheral Nerves intheAdult
https://t.me/med1917
147
peripheral nerve wounds the optimal degradation half-life is about 2weeks, again matching roughly the half-life for the healing process in the transected nerve stump [119]. When the scaffold degraded at a slower rate (tb>>14days), the persisting DRT appeared to interfere with synthesis of the regenerate and scar formed around the scaffold. When the half-life of the DRT was signicantly lower than the half-life of the contractile response (tb<<14days), the DRT had little effect on blocking contraction or scar syn­thesis, and regeneration was not observed [18].
In summary, DRT dramatically blocks contraction while inducing skin regeneration. Scaffolds that are close in struc­ture to DRT but do not block contraction and do not induce regeneration. There is evidence that DRT prevents recruit­ment of MFB and formation of oriented structures of MFB, two processes that characterize spontaneous healing in the adult mammal, over the duration of the normal contraction process.
Discussion andConclusions
The experimental protocols that were used by several inde­pendent investigators to induce synthesis of elements of the skin and peripheral nerves both invitro and invivo were ana­lyzed in an effort to identify the minimal reactants required for organ regeneration. Despite the structural differences between the two organs, the simplest reactants required for induced regeneration of either the skin or peripheral nerves were found to be similar. The empirical evidence supports the conclusion that partial synthesis of either the skin or peripheral nerves requires only the implantation of a scaffold with the requisite structure, appropriately seeded with epi­thelial cells dissociated from the organ of interest. The scaf­fold should possess a minimal density of specic ligands for contractile cells and an optimal persistence time in the insol­uble state [1]. Exogenous reactants utilized widely in many regeneration protocols, notably cytokines and stromal cells (broblasts), were redundant. While the experimental evi­dence derives only from the two organs that have been stud­ied extensively to date in this context, the conclusions reached above may be interpreted as a “trans-organ” approach for future regeneration efforts.
The evidence presented in this chapter shows that severe wounds in several organs in adults heal primarily by contrac­tion, the same mechanism by which the skin and peripheral nerves heal in adults. Contraction blocking in the skin and in peripheral nerves is associated with induced regeneration. The available data suggest, therefore, the possibility that the mechanism of contraction blocking by scaffolds is similar in these two organs. It now becomes possible to seriously con­sider the possibility that the adult organism can be enabled to regenerate most of its organs.
References
1. Yannas IV. Tissue and organ regeneration in adults. NewYork: Springer; 2001.
2. Butler CE, Orgill DP.Simultaneous in vivo regeneration of neo­dermis, epidermis, and basement membrane. Adv Biochem Eng Biotechnol. 2005;94:23–41. https://doi.org/10.1007/b99998.
3. Hatton MP, Rubin PAD.Conjunctival regeneration. Adv Biochem Eng Biotechnol. 2005;94:125–40. https://doi.org/10.1007/
b100002.
4. Zhang M, Yannas IV.Peripheral nerve regeneration. Adv Biochem Eng Biotechnol. 2005;94:67–89. https://doi.org/10.1007/b100000.
5. Mistry AS, Mikos AG. Tissue engineering strategies for bone regeneration. Adv Biochem Eng Biotechnol. 2005;94:1–22.
https://doi.org/10.1007/b99997.
6. Rabkin-Aikawa E, Mayer JEJ, Schoen FJ.Heart valve regenera­tion. Adv Biochem Eng Biotechnol. 2005;94:141–79. https://doi.
org/10.1007/b100003.
7. Takimoto Y, Dixit V, Arthur M, Gitnick G. De novo liver tis­sue formation in rats using a novel collagen-polypropylene scaffold. Cell Transplant. 2003;12(4):413–21. https://doi.
org/10.3727/000000003108746966.
8. Kinner B, Capito RM, Spector M.Regeneration of articular carti­lage. Adv Biochem Eng Biotechnol. 2005;94:91–123. https://doi.
org/10.1007/b100001.
9. Atala A. Regeneration of urologic tissues and organs. Adv Biochem Eng Biotechnol. 2005;94:181–210. https://doi.
org/10.1007/b100004.
10. Verma P, Fawcett J.Spinal cord regeneration. Adv Biochem Eng Biotechnol. 2005;94:43–66. https://doi.org/10.1007/b99999.
11. Canonico S, Campitiello F, Della Corte A, Fattopace A.The use of a dermal substitute and thin skin grafts in the cure of “com­plex” leg ulcers. Dermatol Surg. 2009;35(2):195–200. https://doi.
org/10.1111/j.1524- 4725.2008.34409.x.
12. Clerici G, Caminiti M, Curci V, Quarantiello A, Faglia E.The use of a dermal substitute to preserve maximal foot length in diabetic foot wounds with tendon and bone exposure following urgent sur­gical debridement for acute infection. Int Wound J. 2010;7(3):176–
83. https://doi.org/10.1111/j.1742- 481X.2010.00670.x.
13. Clerici G, Caminiti M, Curci V, Quarantiello A, Faglia E. The use of a dermal substitute (integra) to preserve maximal foot length in a diabetic foot wound with bone and tendon expo­sure following urgent surgical debridement for an acute infec­tion. Int J Low Extrem Wounds. 2009;8(4):209–12. https://doi.
org/10.1177/1534734609350553.
14. Silverstein G. Dermal regeneration template in the surgical management of diabetic foot ulcers: a series of ve cases. J Foot Ankle Surg. 2006;45(1):28–33. https://doi.org/10.1053/j.
jfas.2005.10.005.
15. Iorio ML, Goldstein J, Adams M, Steinberg J, Attinger C. Functional limb salvage in the diabetic patient: the use of a collagen bilayer matrix and risk factors for amputation. Plast Reconstr Surg. 20v11;127(1):260–7. https://doi.org/10.1097/
PRS.0b013e3181f95c4b.
16. Gottlieb M, Furman J.Successful management and surgical clo­sure of chronic and pathological wounds using Integra(R). J Burn Surg Wound Care. 2004;3(1):4.
17. Yannas IV, Burke JF, Orgill DP, Skrabut EM. Wound tissue can utilize a polymeric template to synthesize a functional extension of skin. Science. 1982;215(4529):174–6. https://doi.org/10.1126/
science.7031899.
18. Yannas IV, Lee E, Orgill DP, Skrabut EM, Murphy GF.Synthesis and characterization of a model extracellular matrix that induces partial regeneration of adult mammalian skin. Proc Natl Acad Sci. 1989;86(3):933–7. https://doi.org/10.1073/pnas.86.3.933.
19. Burke JF, Yannas IV, Quinby WC, Bondoc CC, Jung WK. Successful use of a physiologically accept-
148
https://t.me/med1917
A. Z. Yang et al.
able articial skin in the treatment of extensive burn injury. Ann Surg. 1981;194(4):413–28. https://doi.
org/10.1097/00000658- 198110000- 00005.
20. Murphy GF, Orgill DP, Yannas IV. Partial dermal regeneration is induced by biodegradable collagen-glycosaminoglycan grafts. Lab Investig. 1990;62(3):305–13.
21. Compton CC, Butler CE, Yannas IV, Warland G, Orgill DP. Organized skin structure is regenerated in vivo from collagen-GAG matrices seeded with autologous keratino­cytes. J Invest Dermatol. 1998;110(6):908–16. https://doi.
org/10.1046/j.1523- 1747.1998.00200.x.
22. Butler CE, Yannas IV, Compton CC, Correia CA, Orgill DP.Comparison of cultured and uncultured keratinocytes seeded into a collagen-GAG matrix for skin replacements. Br J Plast Surg. 1999;52(2):127–32. https://doi.org/10.1054/bjps.1997.3047.
23. Yannas I, Burke J, Orgill D, Skrabut E.Regeneration of skin fol­lowing closure of deep wounds with a biodegradable template. Trans Soc Biomater. 1982;5:24–7.
24. Yannas I, Orgill D, Skrabut E, Burke J. Skin regeneration with a bioreplaceable polymeric template. In: Gebelein C, edi­tor. Polymeric materials and artical organs. Washington, DC: American Chemical Society; 1984. p.191–7.
25. Yannas I, Orgill D, Silver J, Norregaard T, Zervas N, Schoene W. Polymeric template facilitates regeneration of sciatic nerve across 15mm gap. Trans Soc Biomater. 1985;8:146.
26. Yannas I, Orgill D, Silver J, Norregaard T, Zervas N, Schoene W. Regeneration of sciatic nerve across 15mm gap by use of a polymeric template. In: Gebelein C, editor. Advances in biomedi­cal polymers. NewYork: Plenum Publishing Corporation; 1987. p.1–9.
27. Chang A, Yannas I, Perutz S. Electrophysiological study of recovery of peripheral nerves regenerated by a collagen­glycosaminoglycan copolymer matrix. In: Gebelein C, Dunn R, editors. Progress in biomedical polymers. NewYork, NY: Plenum Publishing Corporation; 1990. p.107–19.
28. Chang A-P, Yannas I.Peripheral nerve regeneration. In: Smith B, Adelman G, editors. Neuroscience year. Boston, MA: Birkhauser;
1992.
29. Chamberlain L, Yannas I, Arrizabalaga A, Hsu H-P, Norregaard T, Spector M. Early peripheral nerve healing in collagen and silicone tube implants: myobroblasts and the cellular response. Biomaterials. 1998;19:1393–403.
30. Chamberlain LJ, Yannas IV, Hsu HP, Strichartz G, Spector M.Collagen-GAG substrate enhances the quality of nerve regen­eration through collagen tubes up to level of autograft. Exp Neurol. 1998;154(2):315–29. https://doi.org/10.1006/exnr.1998.6955.
31. Chamberlain LJ, Yannas IV, Hsu HP, Spector M. Connective tissue response to tubular implants for peripheral nerve regeneration: the role of myobroblasts. J Comp Neurol. 2000;417(4):415–30. https://doi.org/10.1002/
(sici)1096- 9861(20000221)417:4<415::aid- cne3>3.0.co;2- 9.
32. Chamberlain LJ, Yannas IV, Hsu HP, Strichartz GR, Spector M. Near- terminus axonal structure and function following rat sciatic nerve regeneration through a collagen-GAG matrix in a ten-millimeter gap. J Neurosci Res. 2000;60(5):666–77. https://
doi.org/10.1002/(SICI)1097- 4547(20000601)60:5<666::AID­JNR12>3.0.CO;2- 0.
33. Spilker M.Peripheral nerve regeneration through tubular devices.
2000.
34. Hsu WC, Spilker MH, Yannas IV, Rubin PA. Inhibition of conjunctival scarring and contraction by a porous collagen­glycosaminoglycan implant. Invest Ophthalmol Vis Sci. 2000;41(9):2404–11.
35. Goss R.Regeneration versus repair. In: Cohen I, Diegelmann R, Lindblad W, editors. Wound healing: biochemical and clinical aspects. Philadelphia, PA: Saunders; 1992. p.20–39.
36. Martinez-Hernandez A. Repair, regeneration, and brosis. In: Rubin E, Farber J, editors. Pathology. Philadelphia, Pa: Lippincott­Raven; 1998. p.66–95.
37. Burkitt H, Young B, Heath J, Kilgore J.Wheater’s functional his­tology. Edinburgh: Churchill Livingstone; 1993.
38. Vracko R. Basal lamina scaffold-anatomy and signi­cance for maintenance of orderly tissue structure. Am J Pathol. 1974;77(2):314–46. http://www.ncbi.nlm.nih.gov/
pubmed/4614671
39. Bunge RP, Bunge MB. Interrelationship between Schwann cell function and extracellular matrix production. Trends Neurosci. 1983;6:499–505. https://doi.org/10.1016/0166- 2236(83)90235- 7.
40. Fu SY, Gordon T.The cellular and molecular basis of peripheral nerve regeneration. Mol Neurobiol. 1997;14(1–2):67–116. https://
doi.org/10.1007/BF02740621.
41. Haber RM, Hanna W, Ramsay CA, Boxall LB.Cicatricial junc­tional epidermolysis bullosa. J Am Acad Dermatol. 1985;12(5 Pt
1):836–44. https://doi.org/10.1016/s0190- 9622(85)70105- 3.
42. Ikeda K, Oda Y, Tomita K, Nomura S, Nakanishi I. Isolated Schwann cells can synthesize the basement membrane invivo. J Electron Microsc. 1989;38(4):230–4.
43. Stenn K, Malhotra R.Epithelialization. In: Cohen I, Diegelmann R, Lindblad W, editors. Wound healing: biochemical and clinical aspects. Philadelphia, PA: Saunders; 1992. p.115–27.
44. Uitto J, Mauviel A, McGrath J.The dermal-epidermal basement membrane zone in cutaneous wound healing. In: Clark R, edi­tor. The molecular and cellular biology of wound repair. 2nd ed. NewYork, NY: Plenum; 1996. p.513–60.
45. Winter G.Epidermal regeneration studied in the domestic pig. In: Maibach H, Rovee D, editors. Epidermal wound healing. Chicago, IL: Year Book Medical Publishers; 1972. p.71–112.
46. de Medinaceli L, Wyatt RJ, Freed WJ.Peripheral nerve reconnec­tion: mechanical, thermal, and ionic conditions that promote the return of function. Exp Neurol. 1983;81(2):469–87. https://doi.
org/10.1016/0014- 4886(83)90276- 5.
47. Terzis J.Microreconstruction of nerve injuries. Philadelphia, PA: WB Saunders; 1987.
48. Yannas IV. Collagen and gelatin in the solid state. J Macromol Sci Part C. 1972;7(1):49–106. https://doi.
org/10.1080/15321797208068160.
49. Yannas IV, Tzeranis DS, So PTC. Regeneration mechanism for skin and peripheral nerves claried at the organ and molecu­lar scales. Curr Opin Biomed Eng. 2018;6:1–7. https://doi.
org/10.1016/j.cobme.2017.12.002.
50. Agarwal S, Saha S, Balla VK, Pal A, Barui A, Bodhak S.Current developments in 3D bioprinting for tissue and organ regener­ation–a review. Front Mech Eng. 2020;6:589171. https://doi.
org/10.3389/fmech.2020.589171.
51. Wen X, Jiao L, Tan H.MAPK/ERK pathway as a central regulator in vertebrate organ regeneration. Int J Mol Sci. 2022;23(3) https://
doi.org/10.3390/ijms23031464.
52. Ikeda E, Ogawa M, Takeo M, Tsuji T. Functional ectodermal organ regeneration as the next generation of organ replacement therapy. Open Biol. 2019;9(3):190010. https://doi.org/10.1098/
rsob.190010.
53. Pulawska-Czub A, Pieczonka TD, Mazurek P, Kobielak K. The potential of nail mini-organ stem cells in skin, nail and digit tips regeneration. Int J Mol Sci. 2021;22(6) https://doi.org/10.3390/
ijms22062864.
54. Filosa A, Sawamiphak S. Heart development and regeneration­ a multi-organ effort. FEBS J. 2023;290(4):913–30. https://doi.
org/10.1111/febs.16319.
55. Kim SW, Kim YY, Kim H, Ku S-Y.Recent advancements in engi­neered biomaterials for the regeneration of female reproductive organs. Reprod Sci. 2021;28(6):1612–25. https://doi.org/10.1007/
s43032- 021- 00553- y.
8 Regeneration oftheSkin andPeripheral Nerves intheAdult
https://t.me/med1917
149
56. Sriwiriyanont P, Lynch KA, McFarland KL, Supp DM, Boyce ST.Characterization of hair follicle development in engineered skin substitutes. Slominski AT, ed. PLoS One. 2013;8(6):e65664.
https://doi.org/10.1371/journal.pone.0065664.
57. Soller EC, Tzeranis DS, Miu K, So PTC, Yannas IV.Common fea­tures of optimal collagen scaffolds that disrupt wound contraction and enhance regeneration both in peripheral nerves and in skin. Biomaterials. 2012;33(19):4783–91. https://doi.org/10.1016/j.
biomaterials.2012.03.068.
58. Yannas IV, Tzeranis D, So PT.Surface biology of collagen scaf­fold explains blocking of wound contraction and regeneration of skin and peripheral nerves. Biomed Mater. 2015;11(1):14106.
https://doi.org/10.1088/1748- 6041/11/1/014106.
59. Tzeranis DS, Soller EC, Buydash MC, So PTC, Yannas IV. In situ quantication of surface chemistry in porous collagen bio­materials. Ann Biomed Eng. 2016;44(3):803–15. https://doi.
org/10.1007/s10439- 015- 1445- x.
60. Yannas IV, Tzeranis DS, So PTC. Regeneration of injured skin and peripheral nerves requires control of wound contraction, not scar formation. Wound Repair Regen. 2017;25(2):177–91. https://
doi.org/10.1111/wrr.12516.
61. Driver VR, Lavery LA, Reyzelman AM, etal. A clinical trial of Integra template for diabetic foot ulcer treatment. Wound Repair Regen. 2015;23(6):891–900. https://doi.org/10.1111/wrr.12357.
62. Greenwood JE, Dearman BL. Comparison of a sealed, poly­mer foam biodegradable temporizing matrix against Integra® dermal regeneration template in a porcine wound model. J Burn Care Res. 2012;33(1):163–73. https://doi.org/10.1097/
BCR.0b013e318233fac1.
63. Cheshire PA, Herson MR, Cleland H, Akbarzadeh S.Articial der­mal templates: a comparative study of NovoSorb™ Biodegradable temporising Matrix (BTM) and Integra(®) Dermal Regeneration Template (DRT). Burns. 2016;42(5):1088–96. https://doi.
org/10.1016/j.burns.2016.01.028.
64. Banakh I, Cheshire P, Rahman M, etal. A comparative study of engineered dermal templates for skin wound repair in a mouse model. Int J Mol Sci. 2020;21(12) https://doi.org/10.3390/
ijms21124508.
65. Lo CH, Brown JN, Dantzer EJG, etal. Wound healing and der­mal regeneration in severe burn patients treated with NovoSorb® Biodegradable Temporising Matrix: a prospective clinical study. Burns. 2022;48(3):529–38. https://doi.org/10.1016/j.
burns.2021.07.014.
66. Solanki NS, York B, Gao Y, Baker P, Wong She RB.A consecu­tive case series of defects reconstructed using NovoSorb(Ⓡ) Biodegradable Temporising Matrix: initial experience and early results. J Plast Reconstr Aesthet Surg. 2020;73(10):1845–53.
https://doi.org/10.1016/j.bjps.2020.05.067.
67. Li H, Lim P, Stanley E, et al. Experience with NovoSorb® Biodegradable Temporising Matrix in reconstruction of com­plex wounds. ANZ J Surg. 2021;91(9):1744–50. https://doi.
org/10.1111/ans.16936.
68. Janis JE, Steinberg JS.Discussion. Template for skin regenera­tion. Plast Reconstr Surg. 2011;127(Suppl):71S–4S. https://doi.
org/10.1097/PRS.0b013e3182051405.
69. Krarup C, Ibsen A, Ibsen A, etal. Effects of a collagen nerve guide tube in patients with a median or ulnar nerve lesion. In: AAHS Conference Proceedings; 2011.
70. Bertleff MJOE, Meek MF, Nicolai J-PA.A prospective clinical evaluation of biodegradable neurolac nerve guides for sensory nerve repair in the hand. J Hand Surg Am. 2005;30(3):513–8.
https://doi.org/10.1016/j.jhsa.2004.12.009.
71. Haug A.US Food and Drug Administration/Conformit Europe­approved absorbable nerve conduits for clinical repair of periph­eral and cranial nerves. Ann Plast Surg. 2009;62(6):710. https://
doi.org/10.1097/SAP.0b013e31819e0443.
72. Weber RA, Breidenbach WC, Brown RE, Jabaley ME, Mass DP. A randomized prospective study of polyglycolic acid conduits for digital nerve reconstruction in humans. Plast Reconstr Surg. 2000;106(5):1036–8. https://doi.
org/10.1097/00006534- 200010000- 00013.
73. Donoghoe N, Rosson GD, Dellon AL.Reconstruction of the human median nerve in the forearm with the Neurotube. Microsurgery. 2007;27(7):595–600. https://doi.org/10.1002/micr.20408.
74. Ducic I, Maloney CTJ, Dellon AL.Reconstruction of the spinal accessory nerve with autograft or neurotube? Two case reports. J Reconstr Microsurg. 2005;21(1):29–33; discussion 34. https://doi.
org/10.1055/s- 2005- 862777.
75. Chiriac S, Facca S, Diaconu M, Gouzou S, Liverneaux P. Experience of using the bioresorbable copolyester poly(DL­lactide- ε-caprolactone) nerve conduit guide Neurolac™ for nerve repair in peripheral nerve defects: report on a series of 28 lesions. J Hand Surg Eur. 2012;37(4):342–9. https://doi.
org/10.1177/1753193411422685.
76. Costa Serrão de Araújo G, Couto Neto B, Harley Santos Botelho R, Carpi Malta M.Clinical evaluation after peripheral nerve repair with caprolactone neurotube. Hand (N Y). 2017;12(2):168–74.
https://doi.org/10.1177/1558944716643277.
77. Meek MF, Den Dunnen WFA.Porosity of the wall of a Neurolac nerve conduit hampers nerve regeneration. Microsurgery. 2009;29(6):473–8. https://doi.org/10.1002/micr.20642.
78. Gaudin R, Knipfer C, Henningsen A, Smeets R, Heiland M, Hadlock T. Approaches to peripheral nerve repair: genera­tions of biomaterial conduits yielding to replacing autologous nerve grafts in craniomaxillofacial surgery. Biomed Res Int. 2016;2016:3856262. https://doi.org/10.1155/2016/3856262.
79. Stang F, Keilhoff G, Fansa H. Biocompatibility of different nerve tubes. Materials (Basel). 2009;2(4):1480–507. https://doi.
org/10.3390/ma2041480.
80. Masson-Meyers DS, Andrade TAM, Caetano GF, et al. Experimental models and methods for cutaneous wound healing assessment. Int J Exp Pathol. 2020;101(1–2):21–37. https://doi.
org/10.1111/iep.12346.
81. Ferdman AG, Yannas IV.Scattering of light from histologic sec­tions: a new method for the analysis of connective tissue. J Invest Dermatol. 1993;100(5):710–6. https://doi.org/10.1111/1523-
1747.ep12472364.
82. Khorasani H, Zheng Z, Nguyen C, etal. A quantitative approach to scar analysis. Am J Pathol. 2011;178(2):621–8. https://doi.
org/10.1016/j.ajpath.2010.10.019.
83. Ghosh B, Mandal M, Mitra P, Chatterjee J.Attenuation corrected­optical coherence tomography for quantitative assessment of skin wound healing and scar morphology. J Biophotonics. 2021;14(4):e202000357. https://doi.org/10.1002/jbio.202000357.
84. Abrouk M, Gianatasio C, Li Y, etal. An atlas of optical coherence tomography (OCT): elucidating invivo differences of scar types using OCT in order to guide laser treatment parameters. J Clin Aesthet Dermatol. 2022;15(9):30–9.
85. Billingham RE, Russell PS.Studies on wound healing, with spe­cial reference to the phenomenon of contracture in experimental wounds in rabbits’ skin. Ann Surg. 1956;144(6):961–81. https://
doi.org/10.1097/00000658- 195612000- 00005.
86. Kennedy DF, Cliff WJ.A systematic study of wound contraction in mammalian skin. Pathology. 1979;11(2):207–22. https://doi.
org/10.3109/00313027909061947.
87. Ramirez AT, Soroff HS, Schwartz MS, Mooty J, Pearson E, Raben MS.Experimental wound healing in man. Surg Gynecol Obstet. 1969;128(2):283–93.
88. Waite PM. Rearrangement of neuronal responses in the tri­geminal system of the rat following peripheral nerve section. J Physiol. 1984;352:425–45. https://doi.org/10.1113/jphysiol.1984.
sp015301.
150
https://t.me/med1917
A. Z. Yang et al.
89. Aldskogius H, Arvidsson J.Nerve cell degeneration and death in the trigeminal ganglion of the adult rat following peripheral nerve transection. J Neurocytol. 1978;7(2):229–50. https://doi.
org/10.1007/BF01217921.
90. Oppenheimer R, Hinman FJ. Ureteral regeneration: contracture vs. hyperplasia of smooth muscle. J Urol. 1955;74(4):476–84.
https://doi.org/10.1016/S0022- 5347(17)67306- 3.
91. Kiviat MD, Ross R, Ansell JS.Smooth muscle regeneration in the ureter. Electron microscopic and autoradiographic observations. Am J Pathol. 1973;72(3):403–16.
92. Bulut T, Bilsel Y, Yanar H, et al. The effects of beta­aminopropionitrile on colonic anastomosis in rats. J Investig Surg. 2004;17(4):211–9. https://doi.org/10.1080/08941930490472028.
93. Dahners LE, Banes AJ, Burridge KW.The relationship of actin to ligament contraction. Clin Orthop Relat Res. 1986;210:246–51.
94. Wilson CJ, Dahners LE. An examination of the mechanism of ligament contracture. Clin Orthop Relat Res. 1988;227:286–91.
95. Yannas IV, Orgill DP, Burke JF.Template for skin regeneration. Plast Reconstr Surg. 2011;127(Suppl):60S–70S. https://doi.
org/10.1097/PRS.0b013e318200a44d.
96. Greenhalgh DG, Sprugel KH, Murray MJ, Ross R. PDGF and FGF stimulate wound healing in the genetically diabetic mouse. Am J Pathol. 1990;136(6):1235–46.
97. Puolakkainen PA, Twardzik DR, Ranchalis JE, Pankey SC, Reed MJ, Gombotz WR.The enhancement in wound healing by trans­forming growth factor-beta 1 (TGF-beta 1) depends on the topi­cal delivery system. J Surg Res. 1995;58(3):321–9. https://doi.
org/10.1006/jsre.1995.1050.
98. Billingham RE, Reynolds J. Transplantation studies on sheets of pure epidermal epithelium and on epidermal cell suspen­sions. Br J Plast Surg. 1952;5(1):25–36. https://doi.org/10.1016/
s0007- 1226(52)80004- 9.
99. Hansbrough JF, Morgan JL, Greenleaf GE, Bartel R.Composite grafts of human keratinocytes grown on a polyglactin mesh­cultured broblast dermal substitute function as a bilayer skin replacement in full-thickness wounds on athymic mice. J Burn Care Rehabil. 1993;14(5):485–94. https://doi.
org/10.1097/00004630- 199309000- 00001.
100. Cooper ML, Hansbrough JF, Spielvogel RL, Cohen R, Bartel RL, Naughton G. In vivo optimization of a living dermal substitute employing cultured human broblasts on a biodegradable polyg­lycolic acid or polyglactin mesh. Biomaterials. 1991;12(2):243–8.
https://doi.org/10.1016/0142- 9612(91)90207- q.
101. Lorenz HP, Adzick NS.Scarless skin wound repair in the fetus. West J Med. 1993;159(3):350–5. http://www.ncbi.nlm.nih.gov/
pubmed/8236977
102. Mast B, Nelson J, TM K.Tissue repair in mammalian fetus. In: Cohen I, Diegelmann R, Lindblad W, editors. Wound healing: biochemical and clinical aspects. Philadelphia, PA: WB Saunders;
1992.
103. Martin P. Wound healing—aiming for perfect skin regenera­tion. Science. 1997;276(5309):75–81. https://doi.org/10.1126/
science.276.5309.75.
104. Stocum D. Wound repair, regeneration and articial tissues. Austin, TX: RG Landes Co; 1995.
105. Yannas IV, Colt J, Wai YC. Wound contraction and scar syn­thesis during development of the amphibian Rana cates­beiana. Wound repair Regen. 1996;4(1):29–39. https://doi.
org/10.1046/j.1524- 475X.1996.40107.x.
106. Huang J, Heng S, Zhang W, et al. Dermal extracellular matrix molecules in skin development, homeostasis, wound regeneration and diseases. Semin Cell Dev Biol. 2022;128:137–44. https://doi.
org/10.1016/j.semcdb.2022.02.027.
107. Desmoulière A, Chaponnier C, Gabbiani G.Tissue repair, contrac­tion, and the myobroblast. Wound Repair Regen. 2005;13(1):7–
12. https://doi.org/10.1111/j.1067- 1927.2005.130102.x.
108. Frangos J, editor. Physical forces and the mammalian cell. NewYork, NY: Academic Press; 1993.
109. Freyman TM, Yannas IV, Yokoo R, Gibson LJ.Fibroblast contrac­tion of a collagen-GAG matrix. Biomaterials. 2001;22(21):2883–
91. https://doi.org/10.1016/s0142- 9612(01)00034- 5.
110. Freyman TM, Yannas IV, Pek YS, Yokoo R, Gibson LJ. Micromechanics of broblast contraction of a collagen­GAG matrix. Exp Cell Res. 2001;269(1):140–53. https://doi.
org/10.1006/excr.2001.5302.
111. Harley BA, Spilker MH, Wu JW, etal. Optimal degradation rate for collagen chambers used for regeneration of peripheral nerves over long gaps. Cells Tissues Organs. 2004;176(1–3):153–65.
https://doi.org/10.1159/000075035.
112. Racine-Samson L, Rockey DC, Bissell DM.The role of alpha­1beta1 integrin in wound contraction. A quantitative analy­sis of liver myobroblasts in vivo and in primary culture. J Biol Chem. 1997;272(49):30911–7. https://doi.org/10.1074/
jbc.272.49.30911.
113. Rudolph R, Abraham J, Vecchione T, Guber S, Woodward M. Myobroblasts and free silicon around breast implants. Plast Reconstr Surg. 1978;62(2):185–96. https://doi.
org/10.1097/00006534- 197808000- 00006.
114. Davison SP, McCaffrey TV, Porter MN, Manders E. Improved nerve regeneration with neutralization of transforming growth factor-beta1. Laryngoscope. 1999;109(4):631–5. https://doi.
org/10.1097/00005537- 199904000- 00021.
115. Delaere PR, Hardillo J, Hermans R, Van Den Hof B.Prefabrication of composite tissue for improved tracheal reconstruction. Ann Otol Rhinol Laryngol. 2001;110(9):849–60. https://doi.
org/10.1177/000348940111000909.
116. Ehrlich HP, Keefer KA, Myers RL, Passaniti A. Vanadate and the absence of myobroblasts in wound contraction. Arch Surg. 1999;134(5):494–501. https://doi.org/10.1001/
archsurg.134.5.494.
117. Ehrlich HP, Gabbiani G, Meda P. Cell coupling modulates the contraction of broblast-populated collagen lattices. J Cell Physiol. 2000;184(1):86–92. https://doi.org/10.1002/
(SICI)1097- 4652(200007)184:1<86::AID- JCP9>3.0.CO;2- 5.
118. Eyden B. Electron microscopy in the study of myobroblastic lesions. Semin Diagn Pathol. 2003;20(1):13–24.
119. Amano M, Chihara K, Kimura K, et al. Formation of actin stress bers and focal adhesions enhanced by Rho-kinase. Science. 1997;275(5304):1308–11. https://doi.org/10.1126/
science.275.5304.1308.
120. Hall A. Rho GTPases and the actin cytoskeleton. Science. 1998;279(5350):509–14. https://doi.org/10.1126/
science.279.5350.509.
121. Kimura K, Ito M, Amano M, etal. Regulation of myosin phos­phatase by Rho and Rho-associated kinase (Rho-kinase). Science. 1996;273(5272):245–8. https://doi.org/10.1126/
science.273.5272.245.
122. Serini G, Bochaton-Piallat ML, Ropraz P, et al. The bronec­tin domain ED-A is crucial for myobroblastic phenotype induction by transforming growth factor-beta1. J Cell Biol. 1998;142(3):873–81. https://doi.org/10.1083/jcb.142.3.873.
123. Dugina V, Fontao L, Chaponnier C, Vasiliev J, Gabbiani G. Focal adhesion features during myobroblastic differen­tiation are controlled by intracellular and extracellular factors. J Cell Sci. 2001;114(Pt 18):3285–96. https://doi.org/10.1242/
jcs.114.18.3285.