This work was supported by an Artistic and Scholarly Development grant through Illinois Wesleyan University to TS and funded in part by NIH-R01EY022158 (PL).

The strain of eggs used in this protocol was White Leghorn, and all animal procedures were approved by the Institutional Animal Care and Use Committee at Illinois Wesleyan University.
1. Incubation of chick eggs
<ol>
	<li>Keep the eggs at ~10 &#176;C for up to 1 week after they are laid to halt development. When ready to initiate chick embryo development, wipe the entire eggshell with lint-free wipes (see Table of Materials) saturated with room temperature water to remove dirt and debris.</li>
	<li>Ensure the eggshell is sanitized. Wipe down the entire egg surface with lint-free wipes dampened with 70% ethanol. Quickly wipe off the ethanol to dry the egg and avoid ethanol absorption through the eggshell to the embryo.</li>
	<li>Arrange the eggs horizontally on a tray. Mark the top of the egg to denote the expected position of the embryo. Incubate the eggs horizontally, with the rocking function activated, in a 38 &#176;C humidified incubator.</li>
</ol>
2. Windowing the eggs to prepare for membrane dissection
<ol>
	<li>Remove eggs from the incubator on the third day of embryonic development (E3). Sterilize the top of the eggs with lint-free wipes dampened with 70% ethanol. Dry the ethanol from the eggshell surfaces. 
	NOTE: To ensure that development was not delayed during the windowing procedure, 6-12 eggs were removed, and the procedure was quickly carried out on these while the remaining eggs were left in the incubator.</li>
	<li>Position an egg horizontally in a secure egg holder (see Table of Materials). Using the sharp end of dissecting scissors, create a small hole in the top of the eggshell near the pointed end of the egg. 
	NOTE: This hole will facilitate the removal of albumen, which is necessary to drop the yolk and embryo away from the inner eggshell surface. For egg holders, paper-pulp egg filler flats, within which the eggs come shipped, were used.</li>
	<li>Through the hole (Step 2.2.), insert an 18 G beveled hypodermic needle. With the needle pushed to the bottom inner surface of the egg and the bevel-side of the needle facing the pointed end of the egg (e.g., away from the expected location of the yolk and the embryo near the middle of the egg), remove 2-3 mL of albumen from the chicken egg and discard. 
	NOTE: If one&#39;s needle nicks the embryo or its associated vasculature during this step, it will result in blood being aspirated with the albumen. This will result in embryo death. Further, if the yolk is inadvertently aspirated along with the albumen during this step, the embryo will not be viable. In either case, the egg should be discarded if the embryo cannot be immediately used for other purposes.</li>
	<li>Clean the eggshell surface surrounding the hole with lint-free wipes lightly dampened with 70% ethanol and wipe dry. Seal the hole made for removing albumen with clear tape.</li>
	<li>With the sharp end of dissecting scissors, make a second &#34;window&#34; hole in the top of the eggshell at the marking site (Step 1.3.). Ensure that the scissors do not extend too far into the eggshell to avoid contacting and damaging the embryo or embryonic vasculature, which will often be positioned within the egg directly below the site of the second hole.</li>
	<li>Using curved iris forceps, widen the &#34;window&#34; hole to span ~2-3 cm in diameter and serve as a &#34;window&#34; to the developing embryo beneath the shell.
	<ol>
		<li>Insert one end of the forceps into the hole, keeping it parallel to and closely juxtaposed with the eggshell. With the other forceps end positioned outside the eggshell, carefully pinch the two forceps ends together, allowing them to break and remove small pieces of the eggshell. Continue breaking and removing eggshell fragments until there remains a 2-3 cm window that directly overlays the embryo. 
		NOTE: Eggs in which embryos do not lay directly beneath the hole made in Step 2.6. must not be used as the forthcoming membrane dissections would be challenging to complete. Even with rocking the eggs horizontally, about 10% of the eggs are unusable due to the poor positioning of the embryo. These embryos can be used for other purposes.</li>
	</ol>
	</li>
	<li>To limit bacterial contamination, add through the window hole (e.g., into the egg) ~100-200 &#181;L of Ringer&#39;s solution (8 g of NaCl, 0.37 g of KCl, and 0.23 g of CaCl2.2H20 per L of distilled H20) containing Penicillin/Streptomycin antibiotics (50 U/mL of Penicillin and 50 &#181;g/mL of Streptomycin, see Table of Materials).</li>
	<li>Seal the window hole using clear adhesive tape. Perform the egg sealing by aligning a corner of the tape on the long axis of the hole and pressing the tape to the shell ~1-2 cm away from the edge of the hole.
	<ol>
		<li>Continue sealing around the opening until a hanging flap of tape is left on one side. Press the two pieces of tape together, creating a domed shape over the hole, and press the flap of over-hanging tape to the shell to finish sealing the egg. 
		NOTE: Eggs need to be windowed at either E2 or E3. As per experience, windowing prior to E2 results in low embryo viability. Moreover, by E4, the embryo and extraembryonic membranes become attached to the eggshell10, and any attempts to window at E4 or later often result in embryo damage or tearing of extraembryonic blood vessels, with either event leading to the outcome of embryo death.</li>
	</ol>
	</li>
	<li>Return the &#34;windowed&#34; eggs to the incubator for further development. Ensure to keep the eggs horizontal and turn off the incubator&#39;s rocking function.</li>
	<li>Repeat Steps 2.2.-2.9. for each egg.</li>
</ol>
3. Microdissections of the extraembryonic membranes
<ol>
	<li>Remove an E5.5 windowed egg from the incubator. Expose the embryo by cutting the tape away from the window with sterilized dissecting scissors.</li>
	<li>Use a dissecting microscope to observe the embryo and its extraembryonic membranes through the window. If necessary, use scissors or curved iris forceps to widen the window so that the embryo is well-positioned beneath the window, taking care not to damage the embryonic vasculature.
	<ol>
		<li>Add two drops of Ringer&#39;s solution containing Penicillin/Streptomycin antibiotics to hydrate the embryo and sterilize the egg.</li>
	</ol>
	</li>
	<li>Use a dissecting microscope to ensure the embryo is at the proper developmental stage (Hamburger Hamilton stage 27, ~E5.5)11,12 and locate the positions of the amniochorionic membrane (ACM) and the chorioallantoic membrane (CAM). 
	NOTE: At this stage, the embryo is surrounded by the ACM, which comprises the amniotic membrane and overlying chorionic membrane fused and partially covered by the highly-vascularized allantois, which extends from the embryo&#39;s gut region and fuses with the overlaying chorion to form the CAM11,12. The ACM is not heavily vascularized, which enables one to dissect these membranes to expose the embryo without damaging blood vessels and harming the embryo.</li>
	<li>Perform extraembryonic membrane dissections at this stage (E5.5). 
	NOTE: E5.5 is the ideal time to carry out the extraembryonic membrane dissections. Dissecting the membranes earlier (e.g., at E4) before CAM formation reduces embryo accessibility at later stages11. Moreover, at E5.5, the embryo is only partially covered by the highly-vascularized CAM, yet over the next 1-2 days, the CAM quickly envelops and precludes further access to the embryo11,12. For this reason, membrane dissection at E6 or later is challenging as the risk of tearing blood vessels increases.
	<ol>
		<li>Use a pair of sterilized fine forceps to gently grasp the ACM and pull it away from the embryo. Then use sterilized micro-dissecting scissors to cut a hole in the ACM directly above the forelimb that extends from the membrane overlying the forelimb to the membrane overlying the head. 
		NOTE: This step relaxes the chorion and amnion membranes, thus making them easier to grab and further dissect with forceps in the next steps. See Figure 1 for a helpful schematic of how membranes are dissected through the eggshell window.</li>
	</ol>
	</li>
	<li>Use two pairs of fine, sterile forceps to gently grab the amnion in two adjacent positions between the ACM and the CAM (e.g., an area between the cut made above the forelimb and the nearest edge of the CAM).
	<ol>
		<li>Carefully move each pair of forceps, both firmly gripping the amniotic membrane, away from one another, with one pair moving dorsally to the embryo and the other ventrally. 
		NOTE: This motion serves to tear the amnion further while also separating the ACM (which gets pulled in the dorsal direction with respect to the embryo by one pair of forceps) and the CAM (which gets pulled in the ventral direction with respect to the embryo by the other pair of forceps).</li>
		<li>Ensure that the membranes are separated when the CAM no longer covers the embryo and the allantoic artery and vein, which emanate from the embryonic gut to the CAM, are readily apparent.</li>
	</ol>
	</li>
	<li>Use sterilized fine forceps to dissect and remove any remaining amnion membrane covering the embryo. It is most commonly observed that the remaining amnion will partially cover the caudal half of the embryo.
	<ol>
		<li>Using sterilized forceps, grasp the amnion near the mid-cranial region of the embryo and carefully pull the amnion in a caudal direction with respect to the embryo toward the earlier displaced CAM. The embryo will now be fully exposed, and further growth of the CAM will mainly occur away from the developing embryo. 
		NOTE: See Figure 1 for a helpful schematic on how the exposed embryo will appear following membrane dissection. Also, refer to a previously published report11 for helpful schematic diagrams of Steps 3.3.-3.6.</li>
	</ol>
	</li>
	<li>Add a few drops of Ringer&#39;s solution containing Penicillin/Streptomycin antibiotics to hydrate the embryo and sterilize the egg.</li>
	<li>Reseal the window hole using clear tape, as described in Step 2.8. Return the egg to the incubator for further development, keeping the egg horizontal and keeping the incubator&#39;s rocking function inactivated.</li>
	<li>Repeat Steps 3.1.-3.8. for each egg. 
	NOTE: The extraembryonic membrane dissections at E5.5 described above will enable access to the embryo through E7, which is when wounding can be carried out8,9. By E8, the continued growth of the CAM tissue begins to cover the cranial region of the embryo, thus precluding further access to the cornea. If one desires to carry out wounding in older E8-E9 corneas, it is possible to reposition the growing CAM ventrally with respect to the embryo (Step 3.10.). If one wishes to wound at E7, Step 3.10. is not necessary to perform and one may proceed to Step 4, corneal wounding.</li>
	<li>Remove an E7 egg from the incubator whose extraembryonic membranes were previously dissected at E5.5 (Steps 3.1.-3.8.). Grasp with sterilized forceps any available amnion membrane tissues fused to the CAM and gently pull the amnion membrane away from the cranial region of the embryo in a ventral direction with respect to the embryo. 
	&#8203;NOTE: Since the amnionic membrane being displaced away from the embryo is fused to the CAM, the growing and highly vascularized CAM will follow the amnion-grasping forceps and move away from the cranial region. Repeat this step daily to continually displace the CAM away from the embryo until the embryo is at the desired age for wounding.</li>
</ol>
4. Corneal wounding
<ol>
	<li>Obtain an egg from the incubator for wounding at the desired embryonic age, E7-E9. Expose the embryo by cutting the tape away from the window with sterilized dissecting scissors. Add a few drops of Ringer&#39;s solution containing Penicillin/Streptomycin antibiotics to hydrate the embryo and sterilize the egg.</li>
	<li>Use a micro-dissecting knife to make an incision that spans the extent of the cornea of the right eye (due to how the embryo lays in the egg, the left eye is not accessible but can serve as a non-wounded control), which is parallel to and in line with the choroid fissure (Figure 1). The first cut will traverse the corneal epithelium.
	<ol>
		<li>Use the micro-dissecting knife to again lacerate the cornea in the same spot as the first incision 2x more (e.g., three cuts total, with cut 2 and cut 3 occurring along with the same position in the cornea as cut 1)11. The second laceration will traverse the basement membrane, and the third will penetrate the anterior stroma. 
		NOTE: If the embryo has settled under the dissected CAM, one can use sterilized curved iris forceps to carefully move the head out from under the CAM. Position the curved iris forceps beneath the head, making contact with the left side of the head. Cradle the entire head on top of closed curved iris forceps and gently raise the head around and above the CAM. To help with viability, use a similar technique with the curved iris forceps to tuck the embryo back under the CAM after surgery to promote proper growth of the CAM.</li>
	</ol>
	</li>
	<li>Add 3-4 drops of Ringer&#39;s solution containing Penicillin/Streptomycin antibiotics to hydrate the embryo and sterilize the egg.</li>
	<li>Reseal the window hole with clear tape and return to the incubator, leaving the egg horizontal. Allow the embryo to develop and the corneal wound to heal for a desired period (e.g., 0.5-11 days), and then humanely euthanize the embryo by decapitation.</li>
	<li>Use curved iris forceps to harvest the eye from a euthanized embryo floating in a Petri dish of Ringer&#39;s saline solution by gently grasping the eye on its posterior side, where the eye and facial tissue meet, and carefully lifting the whole eye away and free from the facial tissue.
	<ol>
		<li>Use fine forceps to poke a small hole (3-5 cm) in the back of the whole eye and fix the whole eye in 4% paraformaldehyde at 4 &#176;C overnight with mild agitation.</li>
	</ol>
	</li>
</ol>

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The authors have no competing financial interests concerning the information presented in this manuscript.

The chick is an ideal model system for studying fetal, scarless cornea wound repair. Unlike mammals, the chick is easily accessible throughout development using in ovo8&#160;or ex ovo strategies24. The embryonic chick cornea is much larger than rodent corneas, with nearly 50% of the cranial volume dedicated to the eye25, making it highly amenable to physical manipulations such as wounding. Moreover, chicken eggs are readily availabl...

The cornea is the transparent, outer-most tissue of the eye that transmits and refracts light conducive to visual acuity. In the adult cornea, damage or infection to the corneal stroma leads to a rapid and robust wound healing response characterized by keratocyte proliferation, fibrosis, increased inflammation leading to cytokine-induced apoptosis, generation of repair myofibroblasts, and overall remodeling of the extracellular matrix (ECM)1,2. Following injury, such corneal tissue repair results in opaque scar tissue that reduces corneal transparency and occludes the passage of light, thus distorting vision and, in the most severe cases, leading to corneal blindness3. Thus, there is a clear need to develop reliable animal models to address the complexities of wound healing and to identify the cellular and molecular factors responsible for wound closure and tissue regeneration.
To date, most studies examining corneal wound healing have utilized post-natal4 or adult animal models1,2,5,6,7. While these studies have led to a significant advancement in the understanding of the corneal wound healing response and the mechanisms underlying scar formation, the damaged corneal tissues in these healing models fail to fully regenerate, thus limiting their utility for identifying the molecular factors and cellular mechanisms responsible for fully recapitulating corneal morphology and structure post-injury. By contrast, fetal wounds generated with a knife in the embryonic chick cornea possess an intrinsic capacity to heal fully in a scarless fashion8. Specifically, the embryonic chick cornea exhibits nonfibrotic regeneration with the complete recapitulation of the extracellular matrix structure and innervation patterns8,9.
The present protocol describes a sequence of steps involved in wounding the cornea of an embryonic chick in ovo. First, eggs are windowed at early embryonic ages to facilitate access to the embryo. Second, a series of in ovo physical manipulations to the extraembryonic membranes are conducted to ensure access to the eye is maintained through later stages of development, corresponding to when the three cellular layers of the cornea are formed and wounding is desired. Third, linear central cornea incisions penetrating through the corneal epithelium and into the anterior stroma are made using a microsurgical knife. The regeneration process or fully restored corneas can be analyzed for regenerative potential using various cellular and molecular techniques following the wounding procedure.

<table><tbody><tr><td>18 G hypodermic needle</td><td>Fisher Scientific</td><td>14-826-5D</td><td></td></tr><tr><td>30 degree angled microdissecting knife</td><td>Fine Science Tools</td><td>10056-12</td><td></td></tr><tr><td>4&amp;prime;,6-diamidino-2-phenylindole (DAPI)</td><td>Molecular Probes</td><td>D1306</td><td></td></tr><tr><td>5 mL syringe</td><td>Fisher Scientific</td><td>14-829-45</td><td></td></tr><tr><td>Alexa Fluor labelled secondary antibodies</td><td>Molecular Probes</td><td></td><td></td></tr><tr><td>Calcium chloride dihydrate (CaCl&lt;sub&gt;2&lt;/sub&gt;-H&lt;sub&gt;2&lt;/sub&gt;0)</td><td>Sigma</td><td>C8106</td><td></td></tr><tr><td>Chicken egg trays</td><td>GQF</td><td>O246</td><td></td></tr><tr><td>Dissecting Forceps, Fine Tip, Serrated</td><td>VWR</td><td>82027-408</td><td></td></tr><tr><td>Dissecting scissors, sharp tip</td><td>VWR</td><td>82027-578</td><td></td></tr><tr><td>Iris 1 x 2 Teeth Tissue Forceps, Full Curved</td><td>VWR</td><td>100494-908</td><td></td></tr><tr><td>Kimwipes</td><td>Sigma</td><td>Z188956</td><td></td></tr><tr><td>Microdissecting Scissors</td><td>VWR</td><td>470315-228</td><td></td></tr><tr><td>Mouse anti-fibronectin (IgG1)</td><td>Developmental Studies Hybridoma Bank</td><td>B3/D6</td><td></td></tr><tr><td>Mouse anti-laminin (IgG1)</td><td>Developmental Studies Hybridoma Bank</td><td>3H11</td><td></td></tr><tr><td>Mouse antineuron-specific &amp;beta;-tubulin (Tuj1, IgG2a)</td><td>Biolegend</td><td>801213</td><td></td></tr><tr><td>Mouse anti-tenascin (IgG1)</td><td>Developmental Studies Hybridoma Bank</td><td>M1-B4</td><td></td></tr><tr><td>Paraformaldehyde</td><td>Sigma</td><td>158127</td><td></td></tr><tr><td>Penicillin/Streptomycin</td><td>Sigma</td><td>P4333</td><td></td></tr><tr><td>Potassium chloride (KCl)</td><td>Sigma</td><td>P5405</td><td></td></tr><tr><td>Sodium chloride (NaCl)</td><td>Fisher Scientific</td><td>BP358</td><td></td></tr><tr><td>Sportsman 1502 egg incubator</td><td>GQF</td><td>1502</td><td></td></tr><tr><td>Tear by hand packaging (1.88 inch width)</td><td>Scotch</td><td>n/a</td><td></td></tr></tbody></table>

investigating scarless tissue regeneration in embryonic wounded chick corneas

Chick embryonic corneal wounds display a remarkable capacity to fully and rapidly regenerate, whereas adult wounded corneas experience a loss of transparency due to fibrotic scarring. The tissue integrity of injured embryonic corneas is intrinsically restored with no detectable scar formation. Given its accessibility and ease of manipulation, the chick embryo is an ideal model for studying scarless corneal wound repair. This protocol demonstrates the different steps involved in wounding the cornea of an embryonic chick in ovo. First, eggs are windowed at early embryonic ages to access the eye. Second, a series of in ovo physical manipulations to the extraembryonic membranes are conducted to ensure access to the eye is maintained through later stages of development, corresponding to when the three cellular layers of the cornea are formed. Third, linear cornea wounds that penetrate the outer epithelial layer and the anterior stroma are made using a microsurgical knife. The regeneration process or fully restored corneas can be analyzed for regenerative potential using various cellular and molecular techniques following the wounding procedure. Studies to date using this model have revealed that wounded embryonic corneas display activation of keratocyte differentiation, undergo coordinated remodeling of ECM proteins to their native three-dimensional macrostructure, and become adequately re-innervated by corneal sensory nerves. In the future, the potential impact of endogenous or exogenous factors on the regenerative process could be analyzed in healing corneas by using developmental biology techniques, such as tissue grafting, electroporation, retroviral infection, or bead implantation. The current strategy identifies the embryonic chick as a crucial experimental paradigm for elucidating the molecular and cellular factors coordinating scarless corneal wound healing.

Following the earlier dissection of the ACM and CAM at E5.5 to expose the cranial region of the developing embryo, a series of lacerations that spanned the E7 central cornea was made in ovo (Figure 1). An ideal wound to study cornea regeneration occurs following three lacerations, each made in the same location of the cornea. The first laceration traverses the corneal epithelium, while the second and third lacerations penetrate the underlying basement membrane and anterior stroma, r...

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Investigating Scarless Tissue Regeneration in Embryonic Wounded Chick Corneas

The present protocol demonstrates the different steps involved in wounding the cornea of an embryonic chick in ovo. The regenerating or fully restored corneas can be analyzed for regenerative potential using various cellular and molecular techniques following the wounding procedure.&#160;

Chick embryonic corneal wounds display a remarkable capacity to fully and rapidly regenerate, whereas adult wounded corneas experience a loss of ...

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Research

JoVE Journal

Developmental Biology

1.9K Views.  Illinois Wesleyan University. The present protocol demonstrates the different steps involved in wounding the cornea of an embryonic chick in ovo. The regenerating or fully restored corneas can be analyzed for regenerative potential using various cellular and molecular techniques following the wounding procedure. 

Video: Investigating Scarless Tissue Regeneration in Embryonic Wounded Chick Corneas

Establishment of a Clinically Relevant Ex Vivo Mock Cataract Surgery Model for Investigating Epithelial Wound Repair in a Native Microenvironment

The major impediment to understanding how an epithelial tissue executes wound repair is the limited availability of models in which it is possible to follow and manipulate the wound response ex vivo in an environment that closely mimics that of epithelial tissue injury in vivo. This issue was addressed by creating a clinically relevant epithelial ex vivo injury-repair model based on cataract surgery. In this culture model, the response of the lens epithelium to wounding can be followed live in the cells&#8217; native microenvironment, and the molecular mediators of wound repair easily manipulated during the repair process. To prepare the cultures, lenses are removed from the eye and a small incision is made in the anterior of the lens from which the inner mass of lens fiber cells is removed. This procedure creates a circular wound on the posterior lens capsule, the thick basement membrane that surrounds the lens. This wound area where the fiber cells were attached is located just adjacent to a continuous monolayer of lens epithelial cells that remains linked to the lens capsule during the surgical procedure. The wounded epithelium, the cell type from which fiber cells are derived during development, responds to the injury of fiber cell removal by moving collectively across the wound area, led by a population of vimentin-rich repair cells whose mesenchymal progenitors are endogenous to the lens1. These properties are typical of a normal epithelial wound healing response. In this model, as in vivo, wound repair is dependent on signals supplied by the endogenous environment that is uniquely maintained in this ex vivo culture system, providing an ideal opportunity for discovery of the mechanisms that regulate repair of an epithelium following wounding.

Establishment of a Clinically Relevant Ex Vivo Mock Cataract Surgery Model for Investigating Epithelial Wound Repair in a Native Microenvironment

Described here is the establishment of a clinically relevant ex vivo mock cataract surgery model that can be used to investigate mechanisms of the injury response of epithelial tissues within their native microenvironment.

The major impediment to understanding how an epithelial tissue executes wound repair is the limited availability of models in which it is possible to ...

A Method for Lineage Tracing of Corneal Cells Using Multi-color Fluorescent Reporter Mice

Lineage tracing experiments define the origin, fate and behavior of cells in a specific tissue or organism. This technique has been successfully applied for many decades, revealing seminal findings in developmental biology. More recently, it was adopted by stem cell biologists to identify and track different stem cell populations with minimal experimental intervention. The recent developments in mouse genetics, the availability of a large number of mouse strains, and the advancements in fluorescent microscopy allow the straightforward design of powerful lineage tracing systems for various tissues with basic expertise, using commercially available tools. We have recently taken advantage of this powerful methodology to explore the origin and fate of stem cells at the ocular surface using R26R-Confetti mouse. This model offers a multi-color genetic system, for the expression of 4 fluorescent genes in a random manner. Here we describe the principles of this methodology and provide an adaptable protocol for designing lineage tracing experiments; specifically for the corneal epithelium as well as for other tissues.

In this article we describe the principles for designing and performing a multi-color lineage tracing experiment using R26R-Confetti mice. We provide a specific protocol for tracking corneal epithelial cells which can be modified for other tissues of interest.

Lineage tracing experiments define the origin, fate and behavior of cells in a specific tissue or organism. This technique has been successfully applied ...

Adenoviral Gene Therapy for Diabetic Keratopathy: Effects on Wound Healing and Stem Cell Marker Expression in Human Organ-cultured Corneas and Limbal Epithelial Cells

The goal of this protocol is to describe molecular alterations in human diabetic corneas and demonstrate how they can be alleviated by adenoviral gene therapy in organ-cultured corneas. The diabetic corneal disease is a complication of diabetes with frequent abnormalities of corneal nerves and epithelial wound healing. We have also documented significantly altered expression of several putative epithelial stem cell markers in human diabetic corneas. To alleviate these changes, adenoviral gene therapy was successfully implemented using the upregulation of c-met proto-oncogene expression and/or the downregulation of proteinases matrix metalloproteinase-10 (MMP-10) and cathepsin F. This therapy accelerated wound healing in diabetic corneas even when only the limbal stem cell compartment was transduced. The best results were obtained with combined treatment. For possible patient transplantation of normalized stem cells, an example is also presented of the optimization of gene transduction in stem cell-enriched cultures using polycationic enhancers. This approach may be useful not only for the selected genes but also for the other mediators of corneal epithelial wound healing and stem cell function.

An example of adenoviral gene therapy in the human diabetic organ-cultured corneas is presented towards the normalization of delayed wound healing and markedly reduced epithelial stem cell marker expression in these corneas. It also describes the optimization of this process in stem cell-enriched limbal epithelial cultures.

The goal of this protocol is to describe molecular alterations in human diabetic corneas and demonstrate how they can be alleviated by adenoviral gene ...

Combination of Microstereolithography and Electrospinning to Produce Membranes Equipped with Niches for Corneal Regeneration

Corneal problems affect millions of people worldwide reducing their quality of life significantly. Corneal disease can be caused by illnesses such as Aniridia or Steven Johnson Syndrome as well as by external factors such as chemical burns or radiation. Current treatments are (i) the use of corneal grafts and (ii) the use of stem cell expanded in the laboratory and delivered on carriers (e.g., amniotic membrane); these treatments are relatively successful but unfortunately they can fail after 3-5 years. There is a need to design and manufacture new corneal biomaterial devices able to mimic in detail the physiological environment where stem cells reside in the cornea. Limbal stem cells are located in the limbus (circular area between cornea and sclera) in specific niches known as the Palisades of Vogt. In this work we have developed a new platform technology which combines two cutting-edge manufacturing techniques (microstereolithography and electrospinning) for the fabrication of corneal membranes that mimic to a certain extent the limbus. Our membranes contain artificial micropockets which aim to provide cells with protection as the Palisades of Vogt do in the eye.

We report a technique for the fabrication of micropockets within electrospun membranes in which to study cell behavior. Specifically, we describe a combination of microstereolithography and electrospinning for the production of PLGA (Poly(lactide-co-glycolide)) corneal biomaterial devices equipped with microfeatures.

Corneal problems affect millions of people worldwide reducing their quality of life significantly. Corneal disease can be caused by illnesses such as ...

Bioengineering

A Simple Mechanical Procedure to Create Limbal Stem Cell Deficiency in Mouse

Limbal stem cell deficiency (LSCD) is a state of malfunction or loss of limbal epithelial stem cells, after which the corneal epithelium is replaced with conjunctiva. Patients suffer from recurrent corneal defects, pain, inflammation, and loss of vision.
Previously, a murine model of LSCD was described and compared to two other models. The goal was to produce a consistent mouse model of LSCD that both mimics the phenotype in humans and lasts long enough to make it possible to study the disease pathophysiology and to evaluate new treatments. Here, the technique is described in more detail.
A motorized tool with a rotating burr has been designed to remove the rust rings from the corneal surface or to smooth the pterygium bed in patients. It is a suitable device to create the desired LSCD model. It is a readily available, easy-to-use tool with a fine tip that makes it appropriate for working on small eyes, as in mice. Its application prevents unnecessary trauma to the eye and it does not result in unwanted injuries, as often is the case with chemical injury models. As opposed to a blunt scraper, it removes the epithelium with the basement membrane. In this protocol, the limbal area was abraded two times, and then the whole corneal epithelium was shaved from limbus to limbus. To avoid stroma injury, care was taken not to brush the corneal surface once the epithelium was already removed.

The following article provides an easy, reproducible technique to effectively create a sustainable mouse model of limbal stem cell deficiency (LSCD). This animal model is useful in testing and comparing the efficacy of treatments for limbal stem cell diseases.

Limbal stem cell deficiency (LSCD) is a state of malfunction or loss of limbal epithelial stem cells, after which the corneal epithelium is replaced with ...

Medicine

Corneal Epithelial Abrasion with Ocular Burr As a Model for Cornea Wound Healing

The murine cornea provides an excellent model to study wound healing. The cornea is the outermost layer of the eye, and thus is the first defense to injury. In fact, the most common type of eye injury found in clinic is a corneal abrasion. Here, we utilize an ocular burr to induce an abrasion resulting in removal of the corneal epithelium in vivo on anesthetized mice. This method allows for targeted and reproducible epithelial disruption, leaving other areas intact. In addition, we describe the visualization of the abraded epithelium with fluorescein staining and provide concrete advice on how to visualize the abraded cornea. Then, we follow the timeline of wound healing 0, 18, and 72 h after abrasion, until the wound is re-epithelialized. The epithelial abrasion model of corneal injury is ideal for studies on epithelial cell proliferation, migration and re-epithelialization of the corneal layers. However, this method is not optimal to study stromal activation during wound healing, because the ocular burr does not penetrate to the stromal cell layers. This method is also suitable for clinical applications, for example, pre-clinical test of drug effectiveness.

This protocol describes a method to inflict an abrasion to the ocular surface of the mouse, and to follow the wound healing process thereafter. The protocol takes advantage of an ocular burr to partially remove the surface epithelium of the eye in anaesthetized mice.

The murine cornea provides an excellent model to study wound healing. The cornea is the outermost layer of the eye, and thus is the first defense to ...

Ex Vivo Corneal Organ Culture Model for Wound Healing Studies

The cornea has been used extensively as a model system to study wound healing. The ability to generate and utilize primary mammalian cells in two dimensional (2D) and three dimensional (3D) culture has generated a wealth of information not only about corneal biology but also about wound healing, myofibroblast biology, and scarring in general. The goal of the protocol is an assay system for quantifying myofibroblast development, which characterizes scarring. We demonstrate a corneal organ culture ex vivo model using pig eyes. In this anterior keratectomy wound, corneas still in the globe are wounded with a circular blade called a trephine. A plug of approximately 1/3 of the anterior cornea is removed including the epithelium, the basement membrane, and the anterior part of the stroma. After wounding, corneas are cut from the globe, mounted on a collagen/agar base, and cultured for two weeks in supplemented-serum free medium with stabilized vitamin C to augment cell proliferation and extracellular matrix secretion by resident fibroblasts. Activation of myofibroblasts in the anterior stroma is evident in the healed cornea. This model can be used to assay wound closure, the development of myofibroblasts and fibrotic markers, and for toxicology studies. In addition, the effects of small molecule inhibitors as well as lipid-mediated siRNA transfection for gene knockdown can be tested in this system.

A protocol for an ex vivo corneal organ culture model useful for wound healing studies is described. This model system can be used to assess the effects of agents to promote regenerative healing or drug toxicity in an organized 3D multicellular environment.

The cornea has been used extensively as a model system to study wound healing. The ability to generate and utilize primary mammalian cells in two ...

An Epithelial Abrasion Model for Studying Corneal Wound Healing

The cornea is critical for vision, accounting for about two-thirds of the refractive power of the eye. Crucial to the role of the cornea in vision is its transparency. However, due to its external position, the cornea is highly susceptible to a wide variety of injuries that can lead to the loss of corneal transparency and eventual blindness. Efficient corneal wound healing in response to these injuries is pivotal for maintaining corneal homeostasis and preservation of corneal transparency and refractive capabilities. In events of compromised corneal wound healing, the cornea becomes vulnerable to infections, ulcerations, and scarring. Given the fundamental importance of corneal wound healing to the preservation of corneal transparency and vision, a better understanding of the normal corneal wound healing process is a prerequisite to understanding impaired corneal wound healing associated with infection and disease. Toward this goal, murine models of corneal wounding have proven useful in furthering our understanding of the corneal wound healing mechanisms operating under normal physiological conditions. Here, a protocol for creating a central corneal epithelial abrasion in mouse using a trephine and a blunt golf club spud is described. In this model, a 2 mm diameter circular trephine, centered over the cornea, is used to demarcate the wound area. The golf club spud is used with care to debride the epithelium and create a circular wound without damaging the corneal epithelial basement membrane. The resulting inflammatory response proceeds as a well-characterized cascade of cellular and molecular events that are critical for efficient wound healing. This simple corneal wound healing model is highly reproducible and well-published and is now being used to evaluate compromised corneal wound healing in the context of disease.

Here, a protocol for creating a central corneal epithelial abrasion wound in the mouse using a trephine and a blunt golf club spud is described. This corneal wound healing model is highly reproducible and is now being used to evaluate compromised corneal wound healing in the context of diseases.

The cornea is critical for vision, accounting for about two-thirds of the refractive power of the eye. Crucial to the role of the cornea in vision is its ...

Mongolian Gerbils as an Animal Model of Wound Healing

Corneal wound healing studies have been conducted for a long time and have helped to reduce suffering and develop treatments that contribute to improving patients' eye health. Historically, corneal healing has been studied in rodents such as mice and rats, but these models might not completely mimic human disorders. However, information on other rodents such as Mongolian gerbils (Meriones unguiculatus) is scant in corneal research.
Here, we describe a technique to develop a novel animal model for studying corneal healing after photorefractive keratectomy. Due to the limited literature available on the cornea of M. unguiculatus, we also describe a histological analysis of the normal cornea. These research techniques can also be employed in the study of eye diseases because of the similarity between the corneas of Mongolian gerbils and humans in terms of genetics, anatomy, and physiology.

This article describes a new animal model developed to study the anatomy and histology of the cornea and its healing processes. This new animal model uses the Mongolian gerbil, which has a cornea with many similarities to the human cornea.

Corneal wound healing studies have been conducted for a long time and have helped to reduce suffering and develop treatments that contribute to improving ...

Inhibition of Wound Epidermis Formation via Full Skin Flap Surgery During Axolotl Limb Regeneration

Classical experiments in salamander regenerative biology over the last century have long established that the wound epidermis is a crucial signaling structure that forms rapidly post-amputation and is required for limb regeneration. However, methods to study its precise function at the molecular level over the last decades have been limited due to a paucity of precise functional techniques and genomic information available in salamander model systems. Excitingly, the recent plethora of sequencing technologies coupled with the release of various salamander genomes and the advent of functional genetic testing methods, including CRISPR, makes it possible to re-visit these foundational experiments at unprecedented molecular resolution. Here, I describe how to perform the classically developed full skin flap (FSF) surgery in adult axolotls in order to inhibit wound epidermis formation immediately following amputation. The wound epidermis normally forms via distal migration of epithelial cells in the skin proximal to the amputation plane to seal off the wound from the outside environment. The surgery entails immediately suturing full thickness skin (which includes both epidermal and dermal layers) over the amputation plane to hinder epithelial cell migration and contact with the underlying damaged mesenchymal tissues. Successful surgeries result in the inhibition of blastema formation and limb regeneration. By combining this surgery method with contemporary downstream molecular and functional analyses, researchers can begin to uncover the molecular underpinnings of wound epidermis function and biology during limb regeneration.

This article describes how to perform a surgical method to inhibit wound epidermis formation during axolotl limb regeneration by immediately suturing full thickness skin over the amputation plane. This method allows researchers to investigate the functional roles of the wound epidermis during the early stages of limb regeneration.

Classical experiments in salamander regenerative biology over the last century have long established that the wound epidermis is a crucial signaling ...

Investigating Scarless Tissue Regeneration in Embryonic Wounded Chick Corneas

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Rozdziały w tym wideo

Establishment of a Clinically Relevant Ex Vivo Mock Cataract Surgery Model for Investigating Epithelial Wound Repair in a Native Microenvironment

A Method for Lineage Tracing of Corneal Cells Using Multi-color Fluorescent Reporter Mice

Adenoviral Gene Therapy for Diabetic Keratopathy: Effects on Wound Healing and Stem Cell Marker Expression in Human Organ-cultured Corneas and Limbal Epithelial Cells

Combination of Microstereolithography and Electrospinning to Produce Membranes Equipped with Niches for Corneal Regeneration

A Simple Mechanical Procedure to Create Limbal Stem Cell Deficiency in Mouse

Corneal Epithelial Abrasion with Ocular Burr As a Model for Cornea Wound Healing

Ex Vivo Corneal Organ Culture Model for Wound Healing Studies

An Epithelial Abrasion Model for Studying Corneal Wound Healing

Mongolian Gerbils as an Animal Model of Wound Healing

Inhibition of Wound Epidermis Formation via Full Skin Flap Surgery During Axolotl Limb Regeneration