- Research article
- Open Access
Reprogramming of the chick retinal pigmented epithelium after retinal injury
BMC Biologyvolume 12, Article number: 28 (2014)
One of the promises in regenerative medicine is to regenerate or replace damaged tissues. The embryonic chick can regenerate its retina by transdifferentiation of the retinal pigmented epithelium (RPE) and by activation of stem/progenitor cells present in the ciliary margin. These two ways of regeneration occur concomitantly when an external source of fibroblast growth factor 2 (FGF2) is present after injury (retinectomy). During the process of transdifferentiation, the RPE loses its pigmentation and is reprogrammed to become neuroepithelium, which differentiates to reconstitute the different cell types of the neural retina. Somatic mammalian cells can be reprogrammed to become induced pluripotent stem cells by ectopic expression of pluripotency-inducing factors such as Oct4, Sox2, Klf4, c-Myc and in some cases Nanog and Lin-28. However, there is limited information concerning the expression of these factors during natural regenerative processes. Organisms that are able to regenerate their organs could share similar mechanisms and factors with the reprogramming process of somatic cells. Herein, we investigate the expression of pluripotency-inducing factors in the RPE after retinectomy (injury) and during transdifferentiation in the presence of FGF2.
We present evidence that upon injury, the quiescent (p27Kip1+/BrdU-) RPE cells transiently dedifferentiate and express sox2, c-myc and klf4 along with eye field transcriptional factors and display a differential up-regulation of alternative splice variants of pax6. However, this transient process of dedifferentiation is not sustained unless FGF2 is present. We have identified lin-28 as a downstream target of FGF2 during the process of retina regeneration. Moreover, we show that overexpression of lin-28 after retinectomy was sufficient to induce transdifferentiation of the RPE in the absence of FGF2.
These findings delineate in detail the molecular changes that take place in the RPE during the process of transdifferentiation in the embryonic chick, and specifically identify Lin-28 as an important factor in this process. We propose a novel model in which injury signals initiate RPE dedifferentiation, while FGF2 up-regulates Lin-28, allowing for RPE transdifferentiation to proceed.
Several vertebrate species have the capacity to transdifferentiate the retinal pigmented epithelium (RPE) to retina (for reviews, see [1, 2]). In the chick, the process of RPE transdifferentiation was first described based on histological observations . We previously demonstrated that after retina removal from chick eyes at embryonic day (E) 4 to 4.5 (Stage 24 to 25, according to Hamburger and Hamilton Stages ) and in the presence of fibroblast growth factor 2 (FGF2), the RPE loses its pigmentation and transdifferentiates to become a neuroepithelium, co-expressing the retinal progenitor markers Pax6 and Chx10 through FGF/FGF-Receptor (FGFR)/Mitogen-activated protein kinase (MAPK) and extracellular-signal-regulated kinase (ERK) signaling cascade [5, 6]. Concomitantly with RPE transdifferentiation, the transcriptional factor Mitf, an RPE-specific marker, is down-regulated, suggesting a change in cell fate of the injured RPE. The ectopic expression of Mitf is sufficient to inhibit RPE transdifferentiation, likely inhibiting the up-regulation of pax6 expression . During retina regeneration from the RPE, the newly generated neuroepithelium eventually differentiates into all major cell types found in the retina, and the differentiation pattern follows the same order as it does during normal development . The ability of RPE cells to transdifferentiate ceases as embryonic development proceeds beyond E4.5 . However, the ectopic expression of pax6 is sufficient to induce RPE transdifferentiation in the intact developing chick eye up to E14 (Stage 35) . In chick RPE cultures, overexpression of different pro-neural transcriptional factors such as sox2, ash1, ath5, neuroD, neurogenin1, neurogenin3, cath5 and msx2 can promote the transdifferentiation of the RPE into neuronal cells (reviewed in ). By contrast, there are several factors associated with RPE specification, including Mitf, Otx2, Wnt13, BMP, Shh and Activin [6, 8–15]. The inactivation of Wnt/beta-catenin signaling in the embryonic mouse RPE results in down-regulation of RPE-specific factors Mitf and Otx2 and expression of neural retina markers Chx10 and Rx [9, 10].
Recently, it has been demonstrated that somatic mammalian cells can be reprogrammed to become induced pluripotent stem cells by ectopic expression of pluripotency-inducing factors Oct4, Sox2, c-Myc and Klf4 as well as by the combination of Oct4, Sox2, Nanog and the RNA-binding protein Lin-28 [16, 17]. Among all these transcriptional factors, Oct4 (Pou5f1), Nanog and Sox2 are key factors that maintain embryonic stem cell identity . More recently, efficient differentiation of induced pluripotent stem cells into neural retina cells has been demonstrated, suggesting the possibility of using these cells for clinical therapies . Other studies have used a specific set of factors to convert fibroblasts directly into induced neural cells . For example, mouse fibroblasts can be directly converted into induced neural cells by overexpressing Ascl1, Brn2 and Myt1l. However, these induced cells lack the potential to generate diverse neural subtypes . In another work, transient expression of Oct4, Sox2, c-Myc and Klf4 was sufficient to induce transdifferentiation of mouse fibroblasts to neural stem/progenitors cells  that can be expanded and differentiate in multiple neuronal subtypes and glial cells. Although all these methods of reprogramming yield cells with similar characteristics to the target cells, it is still unknown if these reprogrammed cells are able to recapitulate the natural process of differentiation or whether the induced pluripotent stem cells or induced neural cells retain the epigenetic memory of their origin. Importantly, aberrant expression of pluripotency genes, incomplete demethylation of specific promoters, viral integration and, more prominently, cancer [23–26] have been reported as a result of reprogramming. Moreover, from the medical point of view, the possibility to integrate these cells into somatic tissue remains unclear.
As an alternative, the study of transdifferentiation and regeneration could provide important information regarding maintenance of pluripotency, dedifferentiation processes, factors involved in cell reprogramming and integration of the cells in the regenerated tissue . Initial studies have shown that among the pluripotency-inducing factors, sox2, c-myc and klf4 are the common factors expressed during lens and limb regeneration in newts and during fin regeneration and Müller glia dedifferentiation in zebrafish [28–30]. More recently, it was demonstrated that in mammals Lin-28 can enhance tissue repair in several contexts including improved hair regrowth and accelerated regrowth of cartilage, bone and mesenchyme after ear and digit injuries .
Lin-28 is an important regulator of let-7 miRNAs, and it has a functional role in organismal growth and metabolism, tissue development, somatic reprogramming and cancer (reviewed in ). During in vitro differentiation of mouse embryonic carcinoma cells to neural and glial fates, Lin-28 can alter the cell fate independently of let-7; in addition, overexpression of Lin-28 increases neurogenesis in the same cell types . In vitro and in vivo experiments have demonstrated that Lin-28 regulates the translation and stability of a large number of mRNAs including cell cycle regulators, splicing factors, metabolic enzymes and RNA-binding proteins [31, 34–38]. All this evidence strongly suggests that Lin-28 can have a pivotal role in tissue regeneration.
Consistent with this idea, we analyzed the expression of pluripotency-inducing factors, including Lin-28, during RPE transdifferentiation, using the embryonic chick model of retina regeneration. Among all the factors, sox2, c-myc and klf4 were transiently up-regulated in the injured RPE (after retinectomy) along with eye field transcriptional factors, achaete-scute complex homolog 1 (ascl1 also known as chicken achaete-scute homolog (CASH-1)) and differential up-regulation of alterative splice variants of pax6. By contrast, lin-28 was significantly up-regulated only in the presence of FGF2 in retinectomized eyes. Moreover, Lin-28 overexpression in the injured RPE was sufficient to induce RPE transdifferentiation.
These results establish a two-step dedifferentiation process. First, upon injury there is an activation of gene expression for sox2, c-myc and klf4, concomitantly with the up-regulation of eye field transcriptional factors. Second, in the presence of FGF2, lin-28 is up-regulated, suggesting a correlation between the expression of lin-28 and the process of transdifferentiation. Overexpression of Lin-28 in the injured RPE was sufficient to induce RPE transdifferentiation in the absence of an external source of growth factors. To our knowledge, these data provide the first evidence that Lin-28 plays an important role in retina regeneration via RPE transdifferentiation. This is also the first detailed study on the molecular profile of the RPE during the process of dedifferentiation.
Results and discussion
Expression of pluripotency-inducing factors in the ciliary margin and retinal pigmented epithelium
To dissect the possible role of pluripotency-inducing factors during RPE transdifferentiation, we decided first to analyze the expression of these factors in E4 eyes (Stage 24, when retinectomies are performed). The presence of transcripts was analyzed by reverse transcriptase-polymerase chain reaction (RT-PCR) from RNA collected from the ciliary margin or RPE. In order to keep the integrity and specificity of all the tissues collected, we used laser capture microdissection. We found that sox2, c-myc, klf4 and lin-28 mRNAs were expressed in the ciliary margin, while only klf4, c-myc and lin-28 were detected in the RPE (Figure 1A). Consistent with the RT-PCR analysis, immunofluorescence staining demonstrated that Sox2, c-Myc, Klf4 and Lin-28 were present in both the ciliary margin and neuroepithelium (Figure 1B-I and Additional file 1: Figure S1A-D). By contrast, only Klf4, c-Myc and Lin-28 were present in the RPE at E4 and E7 (Figure 1G-I and Additional file 1: Figure S1A,C,D). In agreement with our results, Sox2 has been reported to be expressed in the presumptive neural retina and is down-regulated in the presumptive RPE at E4 to 4.5 (Stage 24 to 25) .
Among these factors, it has been reported that Klf4 plays a critical role in neurogenesis and neural migration during cerebral cortex development in mouse . It could be possible that Klf4 has a similar role in retina development. In chick embryos, klf4 mRNA was detected in the neural folds and in the neural tube at Stages 8 to 9. Later, at Stage 27, klf4 was detected in the face and neck region . In our experiments, we detected Klf4 ubiquitously in the ciliary margin, neuroepithelium and RPE (Figure 1A,C,G and Additional file 1: Figure S1C).
In chicken embryos, Lin-28 is ubiquitously expressed in the presumptive limb primordium at Stages 15 to 16, and in other tissues including the neuroepithelium of the optic cup and in the otic vesicle at E2.5 to 3 (Stages 17 to 18) . In mouse, Lin-28 is present in the retina at embryonic days E8.5 to E17.5 [42, 43]. We detected Lin-28 in the chick ciliary margin, RPE and neuroepithelium at E4 (Stage 24) (Figure 1A,E,I) and at E7 (Additional file 1: Figure S1D), suggesting that the presence of this protein could be necessary for growth and differentiation of these tissues.
Among all the factors controlling the regulatory network in embryonic stem cells, Oct4 and Nanog are considered the ‘key partner core’ of transcriptional regulators (for review see [44, 45]). Expression of the avian homologs of oct4 (cPouV) and nanog was demonstrated early in the developing chick at Stages 8 to 9 . We were unable to detect mRNAs of oct4 and nanog in the ciliary margin or RPE at the embryonic days analyzed, but we did confirm their expression in chick embryos at Stages 8 to 9 (Figure 1A). Although we found the expression of sox2, c-myc and klf4 in the ciliary margin, the absence of oct4 and nanog points out that these cells are not pluripotent but may retain some properties of stem cells. Despite the fact that Sox2, c-Myc, Klf4 and Lin-28 are considered pluripotency-inducing factors when used for reprograming in combination with Oct4 and Nanog, these factors have other functions during eye and retina development [39, 47–50].
In the injured eye, the retinal pigmented epithelium dedifferentiates before entering the cell cycle and expresses sox2, c-myc and klf4
It is known from several organisms, that transdifferentiation occurs by the following steps: transient dedifferentiation, proliferation and differentiation into the new linage [1, 51]. However, the time of dedifferentiation and proliferation is highly dependent on the type of damage and model of regeneration. For example, in zebrafish retina, different damage paradigms including light lesions (acute and chronic), chemical treatments that kill retina neurons (ouabain) and mechanical insults to the retina (needle stabbing) ultimately result in regeneration of the lost neurons by Müller glia transdifferentiation; however, the time at which Müller glia dedifferentiate or enter the cell cycle varies between the treatments. Dedifferentiation events have been reported as early as 4 h for the acute light lesion model, about 15 h for the stabbing model and up to 31 h for chronic light lesion cases. Signs of cells entering the cell cycle have been observed 24 to 72 h post lesion (for reviews see [1, 52, 53]. Interestingly, retina damage caused by different concentrations of ouabain generates extensive cell death of retina neurons and promotes the surviving Müller glia to proliferate robustly within a 3- to 12-day period . During lens regeneration in the newt, the pigmented epithelial cells from the dorsal iris that are responsible for replacing the missing lens express nucleostemin (a stem cell marker) 2 days after lentectomy. This is followed by the loss of pigmentation and cell identity, facilitating the subsequent proliferation that takes place 4 days later . Notably, inhibiting the cell cycle using a Cdk2 inhibitor does not block the process of dedifferentiation .
To better understand and characterize the process of RPE transdifferentiation, we analyzed the proliferative status of the RPE. We performed complete retinectomies in E4 (Stage 24) chick eyes in the presence or absence of FGF2, and the embryos were collected at 6 and 24 hours post-retinectomy (h PR) to examine 5-bromo-2′-deoxyuridine (BrdU) incorporation and the cyclin-dependent kinase inhibitor 1B (p27Kip1) for cell cycle arrest. At 6 h PR, in the absence (retinectomy only) or presence of FGF2, we did not observe BrdU-positive cells in the posterior RPE (Additional file 2: Figure S2A,E). By contrast, a large proportion of p27Kip1-positive cells were found in the posterior RPE at 6 h PR regardless of the presence of FGF2 (Additional file 2: Figure S2B,F), suggesting that at this time point the cells were still arrested in the cell cycle and as a consequence proliferation was blocked. However, BrdU-positive cells were detected in the RPE at 24 h PR only in the presence of FGF2 (Additional file 2: Figure S2G), when the RPE became p27Kip1-negative (Additional file 2: Figure S2H), suggesting that RPE cells had entered the cell cycle. We did not observed BrdU-positive cells in the RPE at 24 h PR in the absence of FGF2 (Additional file 2: Figure S2C) when the RPE was still p27Kip1-positive (Additional file 2: Figure S2D); therefore, FGF2 is necessary for the cell cycle entry, and eventually for RPE transdifferentiation .
To analyze the process of dedifferentiation, we wondered if injury (retinectomy) was sufficient to initiate changes in gene expression of pluripotency-inducing factors, genes associated with the RPE specification, and genes associated with retina progenitors, as well as eye field transcriptional factors. We used the following time points of analysis as a reference, 6 h PR (when the RPE cells were still arrested in the cell cycle, even in the presence of FGF2), 24 h PR (when the RPE cells entered the cell cycle in the presence of FGF2) and 72 h PR (when the RPE transdifferentiates in the presence of FGF2 [5, 6]). mRNA levels for all different genes were evaluated by quantitative RT-PCR (RT-qPCR) using RPE samples collected by laser capture microdissection. Surprisingly, at 6 h PR, we observed activation of gene expression of sox2, c-myc and klf4 and over the basal levels detected in uninjured eyes. However, the expression of sox2 decreased by 72 h PR to the basal levels (P = 0.072, n = 3) (Figure 2A). Although the injury was sufficient to up-regulate sox2, c-myc and klf4 (Figure 2A), which are present in retina progenitors (Figure 1B-D), the absence of the transcripts for oct4 and nanog that are present in embryonic stem cells suggest that the RPE cells do not become pluripotent, but do acquire some plasticity. In agreement with our results, in vitro culture of RPE cells, isolated from adult human donor eyes, showed high levels of c-myc and klf4 compared to human embryonic stem cells, however, oct4 and nanog were not detected by immunostaining or RT-qPCR . Among all the pluripotency-inducing factors, c-Myc, Klf4 and Sox2 are the common factors expressed in regenerating tissues [29, 30, 58]. It is of note that we did not detect expression of oct4 in the RPE before or after injury. Interestingly, in zebrafish, klf4 and oct4 are expressed in the uninjured retina and transiently increase during the process of Müller glia dedifferentiation . Also in zebrafish, the knockdown of morpholino against pou5f1 (homolog to Oct4) impairs fin regeneration, suggesting that Oct4 might be crucial for regeneration in this organism .
The process of RPE dedifferentiation was evidenced by the down-regulation of RPE specification genes mitf and tyr (tyrosinase, a melanin-catalyzing enzyme) concomitantly with an up-regulation of neural retina progenitors ascl1 (also known as CASH-1, ash1) and chx10 (vsx2) (Figure 2B,C).
We also decided to analyze if the dedifferentiated RPE cells go back into the lineage of eye formation. Different factors are crucial for eye formation; the most important are the eye field transcriptional factors that are expressed in the anterior neural plate in the region specified to become the eyes. These eye field transcriptional factors include et, rx1(rx), six3, pax6, lhx2, six6 (optx2) and tll[59–61]. The up-regulation of rx1, six6, lhx2 and six3 (Figure 2B) suggests that the injury was enough to induce a transient dedifferentiation of the RPE and promote these cells to go back to the presumptive optic vesicle stage.
Despite the partial dedifferentiation of the RPE cells, by 72 h in the absence of FGF2 the RPE again acquired its pigmentation (not shown) and mitf expression was recovered at higher levels compared with the uninjured eye (P = 0.016, n = 3) (Figure 2C). Similar to what has been observed in Müller glia transdifferentiation in zebrafish, we observed significant up-regulation of ascl1 (CASH-1), a proneural basic helix-loop-helix transcriptional factor. Importantly, ascl1a, the homolog to chicken ascl1, has been used to reprogram fibroblasts to neurons [21, 62]. We also observed significant up-regulation of rx1, which is related to eye field specification [61, 63] (Figure 2B). The importance of Rx has been demonstrated during retina regeneration in pre-metamorphic Xenopus laevis.
We next evaluated the expression of pax6 transcriptional factor, known to be a master regulator of eye development [65–67]. Different alternative splicing variants of pax6 have been identified in different vertebrates, with pax6 (5a+) and pax6 (5a-) being the most evolutionary conserved [68–70]. The alternative splicing of pax6 transcript generates both forms with the variant 5a + that has an additional 14 amino acid residues inserted in the paired domain, resulting in different specific target genes . In the chick, pax6 is expressed in retinal progenitor cells in early stages of eye development and later in ganglion, horizontal and amacrine cells . To determine whether the expression of both alternative splice variants can be regulated in the injured RPE, we performed RT-qPCR using specific primers for both pax6 (5a+) and pax6 (5a-). Although both variants were up-regulated at 6 h PR, we observed a more prominent up-regulation of pax6 (5a-) at 6 h PR (6.46 ± 0.73 fold-change versus 1.40 ± 0.02 for pax6 (5a+)). By contrast, pax6 (5a+) showed a higher expression at 24 h PR (22.45 ± 0.82 versus 5.5 ± 0.18 fold-change for pax6 (5a-)) (Figure 3). These data suggest that pax6 (5a+) and (5a-) are differentially regulated in the RPE after removing the retina. Interestingly, in the chick, when the optic vesicle is formed, the two splice variants of pax6 are expressed in both the central nervous system and the eye primordium, with the pax6 (5a-) variant being the most abundant . In Xenopus laevis, pax6 is up-regulated in RPE cells soon after removal from the choroid, and this expression is not dependent on FGF2, although the regulation of specific variants has not been explored. In the same study, it was suggested that pax6 expression was triggered by the alteration of the cell-extracellular matrix and/or cell-cell interactions [73, 74]. It is possible that a similar effect can occur in the injured RPE in our system. Interestingly, zebrafish has two paralogs of pax6 (pax6a and pax6b) that are required at different points of neuronal progenitor proliferation after light-damage to the retina .
During mouse brain development, Pax6 (5a+) affects cell proliferation but not neural differentiation. By contrast, the canonical Pax6 (5a-) affects cell proliferation and differentiation [76, 77]. It is possible that during the process of RPE transdifferentiation the alternative splice variants of pax6 observed here have different functions or different gene targets. Collectively, these results suggest that upon retina removal at E4 (Stage 24), the quiescent cells of the RPE dedifferentiate to become progenitor-like cells similar to the cells of the optic vesicle that express the combination of eye field transcriptional factors and the factors sox2, c-myc and klf4. This process is transient and not sustained if no growth factors are present.
FGF2 allows for the sustained transcriptional activity of sox2, c-myc and klf4in retinal pigmented epithelium undergoing reprogramming towards retina progenitors
To analyze the effect on the levels of expression of the pluripotency-inducing factors during the process of RPE transdifferentiation, we performed surgeries at E4 in which FGF2 heparin-coated beads were placed in the optic cup as previously described [5, 6]. Thereafter, the embryos were collected at different times (6, 24 and 72 h PR) and processed for laser capture microdissection. In an attempt to avoid variation in the RPE collection, all samples were collected close to the FGF2 bead (see Methods). The RT-qPCR analysis demonstrated that the expression of sox2 and c-myc was enhanced and sustained up to 72 h, when the RPE is reprogrammed towards retinal progenitors (Figure 4A). We did not observe expression of oct4 and nanog under these conditions. We also evaluated the levels of expression of eye field transcriptional factors and the expression of genes associated with the RPE phenotype (mitf and tyr). Our RT-qPCR experiments demonstrated that the expression of rx1, six6, lhx2 and six3 was sustained at high levels (Figure 4B). In contrast with the expression patterns during injury in the absence of FGF2, the alternative splice variants pax6 5a + and 5a- were up-regulated simultaneously from 6 h to 72 h (Figure 4B). RPE transdifferentiation was confirmed by a significant decrease in expression of mitf and tyr at 72 h PR (Figure 4C). Immunostaining revealed that c-Myc, Sox2, Klf4 and the retina progenitor markers Pax6 and Chx10 were present at 72 h PR in the transdifferentiated RPE (Figure 4D-G). In the absence of FGF2 at 72 h PR, the RPE did not transdifferentiate and remained pigmented, expressing only c-Myc, Klf4 and Lin-28, just as it does during normal development (Additional file 1: Figure S1F-J). As expected, in addition to transdifferentiated RPE, we also observed retina regeneration from the pool of stem/progenitor cells located in the ciliary margin of the chick eye (Figure 4D,F) . Thus, we conclude that FGF2 allows the sustained expression of sox2 and c-myc in retina progenitor cells along with eye field transcriptional factors to complete the transdifferentiation program of the RPE.
In agreement with our results, destruction of photoreceptors by acute light lesions in zebrafish central retina results in Müller glia dedifferentiation 4 to 8 h post-lesion, exemplified by a strong Rx1 immunoreactivity . We found a significant up-regulation of rx1 transcript at 6 h post-injury (h PR) during the transient dedifferentiation of the RPE (Figure 2B). Moreover, at 24 h post-lesion, a percentage of the activated zebrafish Müller glia cells re-enter the cell cycle, just as the chick RPE does in the presence of FGF2 (Additional file 2: Figure S2G,H). Interestingly, Müller glia cells respond by dedifferentiating after local loss of contact with photoreceptors; however, this dedifferentiation is not enough to promote re-entry to the cell cycle. Similarly, it is possible that the loss of contact between the RPE and the retina (after retinectomy) triggers the process of RPE dedifferentiation, or that the process involves an inflammation molecule such as TNFα, as in zebrafish , or even anaphylatoxins such as C3a or interleukins like IL-6, which have been shown to play a role in chick retina regeneration . Taken together, these data suggest that similar mechanism of dedifferentiation and proliferation could be shared between retina regeneration from the RPE and from Müller glia cells.
Overexpression of Lin-28 induces retinal pigmented epithelium transdifferentiation
Previously, it has been shown that Lin-28 is present in the neural tube of mouse embryos, co-localizing with Sox2. Interestingly, constitutive expression of Lin-28 in mouse embryonic carcinoma cells increases neural differentiation . During human stem cell differentiation to neural progenitors, overexpression of Lin-28 rescues the proliferation deficit associated with absence of Sox2, suggesting that Lin-28 is important for proliferation of neural progenitors cells . In zebrafish, upon retinal injury, Müller glia cells express the proneural gene ascl1a along with lin-28, generating a regulatory loop in which ascl1a regulates lin-28, which in turn negatively regulates the miRNA Let-7. Because both sox2 and the ascl1 are expressed during the process of RPE transdifferentiation (Figures 4A,B,E), we decided to investigate the regulation of lin-28 expression in the injured eye and during FGF2-induced transdifferentiation. Interestingly, in comparison with sox2, c-myc and klf4, we found that lin-28 was significantly up-regulated in the presence of FGF2, but not with injury alone (Figure 5A). Consistent with our RT-qPCR results, Lin-28 was detected in the transdifferentiated RPE at 72 h PR showing a cytoplasmic pattern (Figures 5B,C). Given that lin-28 mRNA levels are only up-regulated in the presence of FGF2, it is possible that lin-28 could play a role in completing the transdifferentiation process. Thus, we wondered if lin-28 overexpression could be sufficient to induce RPE transdifferentiation in the absence of FGF2. To address this question, we co-electroporated retinectomized chick eyes with a plasmid containing chicken lin-28 (pCLin28a) and pIRES-GFP (to monitor the electroporated areas, see immunostaining in Figure 5H) or co-electroporation of pcDNA3.1 and pIRES-GFP as controls (Figure 5G), and the embryos were collected 72 h PR. The systematic analysis of histological sections showed a range of effects on the RPE varying from clear thickened depigmented areas to full transdifferentiation (n = 33, 48%, Figure 5I). This range of effects is most likely due to the electroporation efficiency. Unlike the remarkable effects observed with lin-28 overexpression, pIRES-GFP (control plasmid) electroporation did not show evidence of transdifferentiation or lack of pigmentation (Figure 5D,G). Furthermore, overexpression of Lin-28 recapitulated FGF-induced transdifferentiation (compare Figure 5E and F) as well as the amount of transdifferentiated area (Figure 5J, P = 0.2356 comparing Lin-28 and FGF2). Collectively, these results demonstrate that Lin-28 is sufficient to induce RPE transdifferentiation in the absence of an external source of FGF2.
We have identified a series of factors that are up-regulated with injury only (step 1) including the factors sox2, c-myc and klf4 and eye field transcriptional factors. In addition, we have found that lin-28, a pluripotency-inducing factor and a microRNA regulator that is also a critical player in other systems of regeneration, is only up-regulated upon addition of FGF2 (step 2) in the chick RPE after retina removal, at a time where there is no cell proliferation (Figure 6). Finally, we demonstrated that Lin-28 is sufficient to induce RPE transdifferentiation in chick retinectomized eyes in the absence of exogenous FGF2. The conservation of a dedifferentiation molecular profile between regenerative models including retina, lens and limb or fin regeneration is indicative of a common process to reprogram cells to a plastic state, where the cells can be directed to expand and respond to environmental cues in order to differentiate and replace lost cells and tissues.
Chick embryos and surgical procedures
Fertilized Specific Pathogen-Free chicken eggs (Charles River Laboratories, Wilmington, MA, USA) were incubated in a humidified rotating incubator at 38°C. At E4 (Stage 24 ), retinectomies and FGF2 treatments were performed as previously described . Embryos were collected at 6, 24 and 72 h PR and processed for laser capture microdissection, histology and immunofluorescence. For proliferation studies, 10 μl of BrdU (10 μg/ml) solution was dropped over the eye of the embryo 1 h before collection.
Laser capture microdissection
Laser capture microdissection was performed as previously described . Briefly, embryos were collected and infiltrated at 4°C with 6.25%, 12.5% and 25% sucrose for 10, 20 or 30 min, respectively, followed by 2:1 25% sucrose to optimal cutting temperature (OCT) compound (Sakura Finetek, Torrance, CA, USA) for 1 h and frozen in dry ice and methylbutane. Cryosections (12 μm) were collected onto metal-framed polyethylene naphthalate membrane slides (Arcturus, Applied Biosystems, Foster City, CA, USA), fixed in 70% ethanol at -20°C for 30 s, rinsed in cold diethylpyrocarbonate-treated water, stained with hematoxylin (Sigma, St. Louis, MO, USA) for 10 s, and dehydrated in ethanol for 30 s each in 70%, 95% and finally 2 min in 100% ethanol. Laser capture microdissection was performed using a Veritas laser capture microdissection system and software as described previously . Laser microdissected sections were collected in CapSure HS LCM Caps (Molecular Devices, Foster City, CA, USA), and total RNA extraction was performed using PicoPure RNA Isolation Kit (Arcturus, Applied Biosystems) including a treatment with DNase I (RNase-Free DNase Set; Qiagen, Darmstadt, Germany). The quality and quantity of RNA were determined using an Agilent RNA 6000 Pico LabChip (Agilent 2100 Bioanalyzer; Agilent Technologies, Santa Clara, CA, USA). Five nanograms of total RNA with an RNA integrity number > 8 were amplified using Ovation Pico WTA System V2 (NuGEN, San Carlo, CA, USA) according to the manufacturer’s instructions, to generate the Single Primer Isothermal Amplification (SPIA) cDNA. Finally, SPIA cDNA was purified using QIAquick PCR Purification Kit (Qiagen) and quantified using a Nanodrop ND-100 spectrophotometer (Thermo Fisher Scientific, Kalamazoo, MI, USA).
Total RNA was extracted from Stage 8 whole embryos using NucleoSpin RNA II isolation Kit (Macherey-Nagel, Düren, Germany) following the manufacture’s protocol. The quality and quantity of RNA were determined using Agilent RNA Nano LabChip (Agilent 2100 Bioanalyzer; Agilent Technologies). Approximately 300 ng of total RNA with a an RNA integrity number > 8 were used for cDNA synthesis using ImProm-II Reverse Transcription System (Promega, Madison, WI, USA) and random-primer hexamers according to the manufacturer’s instructions. For CM and RPE, the amplified SPIA cDNA (50 ng) was used as a template in the PCR reactions. All PCR reactions were performed using PlatinumTaq DNA polymerase (Invitrogen, Grand Island, NY, USA) and the intron-spanning primers are listed in Additional file 3: Table S1. Amplification conditions included denaturation at 95°C for 1 min, annealing at 55°C for 2 min, and extension at 72°C for 30 s. All the RT-PCR reactions were run from at least three independent biological samples and the fragments were gel-purified and sequenced to confirm the specificity of the sequence.
RT-qPCR was performed using a 20 μl mixture containing 5 μl (4 ng) SPIA cDNA, 10 μl 2× SYBR Green/Fluorescein qPCR Master Mix (SABiosciences, Qiagen, MD, USA), and a 500 nM final concentration of the primers. Splice junction-specific primers were designed using Primer 3 (v 4.0) available in  and were optimized following guidelines for RT-qPCR experiments (amplification efficiency and melting curves) . Primers sequences and Ensembl or GenBank identification numbers are provided in Additional file 3: Table S2. Amplifications reactions were performed in triplicate using an iCycler (BioRad, Hercules, CA, USA). The cycling conditions included 10 min polymerase activation at 95°C and 35 cycles of 15 s at 95°C and 1 min at 60°C, followed by a dissociation run from 65°C to 95°C for melting curve analysis. The comparative cycle at threshold (2-ΔΔCt) and an unpaired Student’s t-test analysis were used to determine relative changes in transcript levels compared to gapdh mRNA levels as previously reported  using SigmaPlot 8.0 Software. All analyses were performed in triplicate with at least three independent biological samples.
Antibodies against Sox-2 (1:100), c-Myc (1:50) and Lin-28 (1:100) were purchased from Santa Cruz Biotechnology. Antibody against Klf4 (1:100) was purchased from Aviva Systems Biology (San Diego, CA, USA). Antibodies against Mitf (1:500), GFP (1:50) and BrdU (1:50) were purchased from Abcam (Cambridge, MA, USA). Antibody against Pax-6 (1:10) was obtained from the Developmental Studies Hybridoma Bank (Iowa City, IA, USA). Anti-Chx-10 (1:250) antibody was purchased from ExAlpha (Shirley, MA, USA). Antibody against p27Kip1 (1:50) was obtained from BD Biosciences (Franklin Lakes, NJ, USA). All secondary antibodies were purchased from Molecular Probes (Grand Island, NY, USA) and used at 1:100 dilution.
Embryos were fixed in 4% paraformaldehyde in PBS for 4 h at room temperature, equilibrated in 30% sucrose, embedded in OCT compound (Sakura Finetek), and sectioned at 12 μm. For the p27Kip1 antibody, tissues were fixed in 10% neutral buffered formalin (Thermo Scientific), embedded in paraffin, sectioned, and deparaffinized followed by 30 min antigen retrieval. Sections were permeabilized with 1% saponin in PBS or 15 min in 2 N HCl in PBS for BrdU immunostaining and blocked with 10% goat or donkey serum and incubated overnight at 4°C with the primary antibody. Sections were incubated in secondary antibody and coverslipped with Vectashield (Vector Laboratories, Burlingame, CA, USA). Confocal images (size 1,024 × 1,024) were collected sequentially on a Zeiss 710 Laser Scanning Confocal System (Jena, Germany) using a × 20/0.80 Numeric Aperture (NA) = 0.55 WD objective lens or EC Plan-Neofluar. Results were confirmed using three different biological samples.
Lin-28a construct and in ovo electroporation
Chicken Lin-28a was cloned from a Stage 14 embryo as previously described  and the cDNA was synthetized as described in the RT-PCR section using the primers described in Additional file 3: Table S3. The PCR product was gel-purified and cloned in pDrive plasmid to generate pDlin28a plasmid (Qiagen). Thereafter, a HindIII/BamHI fragment of 895 base pairs from pDlin28a was cloned using the same restriction sites in pcDNA3.1+ (Invitrogen) to generate pCLin28a. T7 primer was used to confirm the integrity of the Lin-28a sequence. Electroporations were performed 1 h PR by injecting 3 μl of a mixture of pCLin28a and pIRES-GFP (1:1, 3 μg each) or 3 μl of a mixture of pcDNA3.1 and pIRES-GFP as controls at the same concentration. The injections were performed using a Pico-injector system PLI-100 (Harvard Apparatus, Holliston, MA, USA) and glass capillary needles. Thereafter, a gold-plated wire electrode (In Ovo gene model 512; BTX Technologies inc., Bent, Holliston, MA, USA), used as an anode, was placed in the ventral border of the eye and a platinum and iridium electrode (FHC Inc., Bowdoinham, ME, USA), used as cathode, was inserted on the top of the brain. Three square pulses of 15 V of 50 ms length and at 950 ms intervals were applied using an ECM 830 electroporator (BTX Technologies, Inc.). The window on the shell was sealed and the embryos were returned to the incubator and collected 72 h post-electroporation and processed for immunohistochemistry and histology.
Histology and quantification
Embryos used for histological analysis were fixed in Bouin’s fixative (Ricca Chemical Company, Arlington, TX, USA), embedded in paraffin, sectioned at 12 μm, stained with hematoxylin and eosin, and photographed using an Olympus BX-51 microscope (Tokio, Japan). To quantify the amount of transdifferentiated RPE, we analyzed the area from three histological sections of four different eyes (12 sections). Images were captured using an Olympus camera and Magnafire image capture software and processed using ImageJ software available in . The transdifferentiated area was calculated using the free hand tool and a two-tailed permutation test for comparing means using R version 3.0.
fibroblast growth factor
- h PR:
optimal cutting temperature
polymerase chain reaction
quantitative polymerase chain reaction
single primer isothermal amplification
tumor necrosis factor alpha.
Barbosa-Sabanero K, Hoffmann A, Judge C, Lightcap N, Tsonis PA, Del Rio-Tsonis K: Lens and retina regeneration: new perspectives from model organisms. Biochem J. 2012, 447: 321-334. 10.1042/BJ20120813.
Fuhrmann S, Zou C, Levine EM: Retinal pigment epithelium development, plasticity, and tissue homeostasis. Exp Eye Res. 2013, [Epub ahead of print]
Coulombre JL, Coulombre AJ: Regeneration of neural retina from the pigmented epithelium in the chick embryo. Dev Biol. 1965, 12: 79-92. 10.1016/0012-1606(65)90022-9.
Hamburger VHH: A series of normal stages in the development of the chick embryo. J Morphol. 1951, 88: 49-92. 10.1002/jmor.1050880104.
Spence JR, Madhavan M, Ewing JD, Jones DK, Lehman BM, Del Rio-Tsonis K: The hedgehog pathway is a modulator of retina regeneration. Development. 2004, 131: 4607-4621. 10.1242/dev.01298.
Spence JR, Madhavan M, Aycinena JC, Del Rio-Tsonis K: Retina regeneration in the chick embryo is not induced by spontaneous Mitf downregulation but requires FGF/FGFR/MEK/Erk dependent upregulation of Pax6. Mol Vis. 2007, 13: 57-65.
Azuma N, Tadokoro K, Asaka A, Yamada M, Yamaguchi Y, Handa H, Matsushima S, Watanabe T, Kida Y, Ogura T, Torri M, Shimamura K, Nakafuku M: Transdifferentiation of the retinal pigment epithelia to the neural retina by transfer of the Pax6 transcriptional factor. Hum Mol Genet. 2005, 14: 1059-1068. 10.1093/hmg/ddi098.
Sakami S, Hisatomi O, Sakakibara S, Liu J, Reh TA, Tokunaga F: Downregulation of Otx2 in the dedifferentiated RPE cells of regenerating newt retina. Brain Res Dev Brain Res. 2005, 155: 49-59. 10.1016/j.devbrainres.2004.11.008.
Fujimura N, Taketo MM, Mori M, Korinek V, Kozmik Z: Spatial and temporal regulation of Wnt/beta-catenin signaling is essential for development of the retinal pigment epithelium. Dev Biol. 2009, 334: 31-45. 10.1016/j.ydbio.2009.07.002.
Westenskow P, Piccolo S, Fuhrmann S: Beta-catenin controls differentiation of the retinal pigment epithelium in the mouse optic cup by regulating Mitf and Otx2 expression. Development. 2009, 136: 2505-2510. 10.1242/dev.032136.
Sakami S, Etter P, Reh TA: Activin signaling limits the competence for retinal regeneration from the pigmented epithelium. Mech Dev. 2008, 125: 106-116. 10.1016/j.mod.2007.10.001.
Fuhrmann S, Levine EM, Reh TA: Extraocular mesenchyme patterns the optic vesicle during early eye development in the embryonic chick. Development. 2000, 127: 4599-4609.
Muller F, Rohrer H, Vogel-Hopker A: Bone morphogenetic proteins specify the retinal pigment epithelium in the chick embryo. Development. 2007, 134: 3483-3493. 10.1242/dev.02884.
Perron M, Boy S, Amato MA, Viczian A, Koebernick K, Pieler T, Harris WA: A novel function for Hedgehog signalling in retinal pigment epithelium differentiation. Development. 2003, 130: 1565-1577. 10.1242/dev.00391.
Zhang XM, Yang XJ: Temporal and spatial effects of Sonic hedgehog signaling in chick eye morphogenesis. Dev Biol. 2001, 233: 271-290. 10.1006/dbio.2000.0195.
Takahashi K, Tanabe K, Ohnuki M, Narita M, Ichisaka T, Tomoda K, Yamanaka S: Induction of pluripotent stem cells from adult human fibroblasts by defined factors. Cell. 2007, 131: 861-872. 10.1016/j.cell.2007.11.019.
Yu J, Vodyanik MA, Smuga-Otto K, Antosiewicz-Bourget J, Frane JL, Tian S, Nie J, Jonsdottir GA, Ruotti V, Slukvin II, Thomson JA: Induced pluripotent stem cell lines derived from human somatic cells. Science. 2007, 318: 1917-1920. 10.1126/science.1151526.
Chan YS, Yang L, Ng HH: Transcriptional regulatory networks in embryonic stem cells. Prog Drug Res. 2011, 67: 239-252.
Cramer AO, MacLaren RE: Translating induced pluripotent stem cells from bench to bedside: application to retinal diseases. Curr Gene Ther. 2013, 13: 139-151. 10.2174/1566523211313020008.
Yang N, Ng YH, Pang ZP, Sudhof TC, Wernig M: Induced neuronal cells: how to make and define a neuron. Cell Stem Cell. 2011, 9: 517-525. 10.1016/j.stem.2011.11.015.
Vierbuchen T, Ostermeier A, Pang ZP, Kokubu Y, Sudhof TC, Wernig M: Direct conversion of fibroblasts to functional neurons by defined factors. Nature. 2010, 463: 1035-1041. 10.1038/nature08797.
Kim J, Efe JA, Zhu S, Talantova M, Yuan X, Wang S, Lipton SA, Zhang K, Ding S: Direct reprogramming of mouse fibroblasts to neural progenitors. Proc Natl Acad Sci U S A. 2011, 108: 7838-7843. 10.1073/pnas.1103113108.
Ohnishi K, Semi K, Yamamoto T, Shimizu M, Tanaka A, Mitsunaga K, Okita K, Osafune K, Arioka Y, Maeda T, Soejima H, Moriwaki H, Yamanaka S, Woltjen K, Yamada Y: Premature termination of reprogramming in vivo leads to cancer development through altered epigenetic regulation. Cell. 2014, 156: 663-677. 10.1016/j.cell.2014.01.005.
Sommer CA, Christodoulou C, Gianotti-Sommer A, Shen SS, Sailaja BS, Hezroni H, Spira A, Meshorer E, Kotton DN, Mostoslavsky G: Residual expression of reprogramming factors affects the transcriptional program and epigenetic signatures of induced pluripotent stem cells. PLoS One. 2012, 7: e51711-10.1371/journal.pone.0051711.
Wang T, Wu H, Li Y, Szulwach KE, Lin L, Li X, Chen IP, Goldlust IS, Chamberlain SJ, Dodd A, Gong H, Ananiev G, Han JW, Yoon YS, Rudd MK, Yu M, Song CX, He C, Chang Q, Warren ST, Jin P: Subtelomeric hotspots of aberrant 5-hydroxymethylcytosine-mediated epigenetic modifications during reprogramming to pluripotency. Nat Cell Biol. 2013, 15: 700-711. 10.1038/ncb2748.
Zhou W, Wang K, Ruan W, Bo Z, Liu L, Cao Z, Chai L, Cao G: Higher methylation in genomic DNA indicates incomplete reprogramming in induced pluripotent stem cells. Cell Reprogram. 2012, 15: 92-99.
Knapp D, Tanaka EM: Regeneration and reprogramming. Curr Opin Genet Dev. 2012, 22: 485-493. 10.1016/j.gde.2012.09.006.
Christen B, Robles V, Raya M, Paramonov I, Izpisua Belmonte JC: Regeneration and reprogramming compared. BMC Biol. 2010, 8: 5-10.1186/1741-7007-8-5.
Ramachandran R, Fausett BV, Goldman D: Ascl1a regulates Muller glia dedifferentiation and retinal regeneration through a Lin-28-dependent, let-7 microRNA signalling pathway. Nat Cell Biol. 2010, 12: 1101-1107. 10.1038/ncb2115.
Maki N, Suetsugu-Maki R, Tarui H, Agata K, Del Rio-Tsonis K, Tsonis PA: Expression of stem cell pluripotency factors during regeneration in newts. Dev Dyn. 2009, 238: 1613-1616. 10.1002/dvdy.21959.
Shyh-Chang N, Zhu H, Yvanka De Soysa T, Shinoda G, Seligson MT, Tsanov KM, Nguyen L, Asara JM, Cantley LC, Daley GQ: Lin28 enhances tissue repair by reprogramming cellular metabolism. Cell. 2013, 155: 778-792. 10.1016/j.cell.2013.09.059.
Shyh-Chang N, Daley GQ: Lin28: primal regulator of growth and metabolism in stem cells. Cell Stem Cell. 2013, 12: 395-406. 10.1016/j.stem.2013.03.005.
Balzer E, Heine C, Jiang Q, Lee VM, Moss EG: LIN28 alters cell fate succession and acts independently of the let-7 microRNA during neurogliogenesis in vitro. Development. 2010, 137: 891-900. 10.1242/dev.042895.
Peng S, Chen LL, Lei XX, Yang L, Lin H, Carmichael GG, Huang Y: Genome-wide studies reveal that Lin28 enhances the translation of genes important for growth and survival of human embryonic stem cells. Stem Cells. 2011, 29: 496-504. 10.1002/stem.591.
Zhu H, Shyh-Chang N, Segre AV, Shinoda G, Shah SP, Einhorn WS, Takeuchi A, Engreitz JM, Hagan JP, Kharas MG, Urbach A, Thornton JE, Triboulet R, Gregory RI, Altshuler D, Daley GQ: The Lin28/let-7 axis regulates glucose metabolism. Cell. 2011, 147: 81-94. 10.1016/j.cell.2011.08.033.
Li N, Zhong X, Lin X, Guo J, Zou L, Tanyi JL, Shao Z, Liang S, Wang LP, Hwang WT, Katsaros D, Montone K, Zhao X, Zhang L: Lin-28 homologue A (LIN28A) promotes cell cycle progression via regulation of cyclin-dependent kinase 2 (CDK2), cyclin D1 (CCND1), and cell division cycle 25 homolog A (CDC25A) expression in cancer. J Biol Chem. 2012, 287: 17386-17397. 10.1074/jbc.M111.321158.
Wilbert ML, Huelga SC, Kapeli K, Stark TJ, Liang TY, Chen SX, Yan BY, Nathanson JL, Hutt KR, Lovci MT, Kazan H, Vu AQ, Massirer KB, Morris Q, Hoon S, Yeo GW: LIN28 binds messenger RNAs at GGAGA motifs and regulates splicing factor abundance. Mol Cell. 2012, 48: 195-206. 10.1016/j.molcel.2012.08.004.
Hafner M, Max KE, Bandaru P, Morozov P, Gerstberger S, Brown M, Molina H, Tuschl T: Identification of mRNAs bound and regulated by human LIN28 proteins and molecular requirements for RNA recognition. RNA. 2013, 19: 613-626. 10.1261/rna.036491.112.
Ishii Y, Weinberg K, Oda-Ishii I, Coughlin L, Mikawa T: Morphogenesis and cytodifferentiation of the avian retinal pigmented epithelium require downregulation of Group B1 Sox genes. Development. 2009, 136: 2579-2589. 10.1242/dev.031344.
Qin S, Zhang CL: Role of Kruppel-like factor 4 in neurogenesis and radial neuronal migration in the developing cerebral cortex. Mol Cell Biol. 2012, 32: 4297-4305. 10.1128/MCB.00838-12.
Antin PB, Pier M, Sesepasara T, Yatskievych TA, Darnell DK: Embryonic expression of the chicken Kruppel-like (KLF) transcription factor gene family. Dev Dyn. 2010, 239: 1879-1887. 10.1002/dvdy.22318.
Yokoyama S, Hashimoto M, Shimizu H, Ueno-Kudoh H, Uchibe K, Kimura I, Asahara H: Dynamic gene expression of Lin-28 during embryonic development in mouse and chicken. Gene Expr Patterns. 2008, 8: 155-160. 10.1016/j.gep.2007.11.001.
Yang DH, Moss EG: Temporally regulated expression of Lin-28 in diverse tissues of the developing mouse. Gene Expr Patterns. 2003, 3: 719-726. 10.1016/S1567-133X(03)00140-6.
Jean C, Aubel P, Soleihavoup C, Bouhallier F, Voisin S, Lavial F, Pain B: Pluripotent genes in avian stem cells. Dev Growth Differ. 2013, 55: 41-51. 10.1111/dgd.12021.
Jaenisch R, Young R: Stem cells, the molecular circuitry of pluripotency and nuclear reprogramming. Cell. 2008, 132: 567-582. 10.1016/j.cell.2008.01.015.
Lavial F, Acloque H, Bertocchini F, Macleod DJ, Boast S, Bachelard E, Montillet G, Thenot S, Sang HM, Stern CD, Samarut J, Pain B: The Oct4 homologue PouV and Nanog regulate pluripotency in chicken embryonic stem cells. Development. 2007, 134: 3549-3563. 10.1242/dev.006569.
La Torre A, Georgi S, Reh TA: Conserved microRNA pathway regulates developmental timing of retinal neurogenesis. Proc Natl Acad Sci U S A. 2013, 110: E2362-E2370. 10.1073/pnas.1301837110.
Matsushima D, Heavner W, Pevny LH: Combinatorial regulation of optic cup progenitor cell fate by SOX2 and PAX6. Development. 2011, 138: 443-454. 10.1242/dev.055178.
Moore DL, Blackmore MG, Hu Y, Kaestner KH, Bixby JL, Lemmon VP, Goldberg JL: KLF family members regulate intrinsic axon regeneration ability. Science. 2009, 326: 298-301. 10.1126/science.1175737.
Xue XY, Harris WA: Using myc genes to search for stem cells in the ciliary margin of the Xenopus retina. Dev Neurobiol. 2012, 72: 475-490. 10.1002/dneu.20887.
Henry JJ, Tsonis PA: Molecular and cellular aspects of amphibian lens regeneration. Prog Retin Eye Res. 2010, 29: 543-555. 10.1016/j.preteyeres.2010.07.002.
Gorsuch RA, Hyde DR: Regulation of Muller glial dependent neuronal regeneration in the damaged adult zebrafish retina. Exp Eye Res. 2013, [Epub ahead of print]
Lenkowski JR, Raymond PA: Muller glia: Stem cells for generation and regeneration of retinal neurons in teleost fish. Prog Retin Eye Res. 2014, [Epub ahead of print]
Sherpa T, Lankford T, McGinn TE, Hunter SS, Frey RA, Sun C, Ryan M: Robison BD. 2014, Stenkamp DL: Retinal regeneration is facilitated by the presence of surviving neurons. Dev Neurobiol, [Epub ahead of print]
Maki N, Takechi K, Sano S, Tarui H, Sasai Y, Agata K: Rapid accumulation of nucleostemin in nucleolus during newt regeneration. Dev Dyn. 2007, 236: 941-950. 10.1002/dvdy.21027.
Tsonis PA, Madhavan M, Call MK, Gainer S, Rice A, Del Rio-Tsonis K: Effects of a CDK inhibitor on lens regeneration. Wound Repair Regen. 2004, 12: 24-29. 10.1111/j.1067-1927.2004.012107.x.
Salero E, Blenkinsop TA, Corneo B, Harris A, Rabin D, Stern JH, Temple S: Adult human RPE can be activated into a multipotent stem cell that produces mesenchymal derivatives. Cell Stem Cell. 2012, 10: 88-95. 10.1016/j.stem.2011.11.018.
Rao N, Jhamb D, Milner DJ, Li B, Song F, Wang M, Voss SR, Palakal M, King MW, Saranjami B, Nye HL, Cameron JA, Stocum DL: Proteomic analysis of blastema formation in regenerating axolotl limbs. BMC Biol. 2009, 7: 83-10.1186/1741-7007-7-83.
Graw J: Eye development. Curr Top Dev Biol. 2010, 90: 343-386.
Sinn R, Wittbrodt J: An eye on eye development. Mech Dev. 2013, 130: 347-358. 10.1016/j.mod.2013.05.001.
Zuber ME, Gestri G, Viczian AS, Barsacchi G, Harris WA: Specification of the vertebrate eye by a network of eye field transcription factors. Development. 2003, 130: 5155-5167. 10.1242/dev.00723.
Son EY, Ichida JK, Wainger BJ, Toma JS, Rafuse VF, Woolf CJ, Eggan K: Conversion of mouse and human fibroblasts into functional spinal motor neurons. Cell Stem Cell. 2011, 9: 205-218. 10.1016/j.stem.2011.07.014.
Chuang JC, Raymond PA: Zebrafish genes rx1 and rx2 help define the region of forebrain that gives rise to retina. Dev Biol. 2001, 231: 13-30. 10.1006/dbio.2000.0125.
Martinez-De Luna RI, Kelly LE, El-Hodiri HM: The Retinal Homeobox (Rx) gene is necessary for retinal regeneration. Dev Biol. 2011, 353: 10-18. 10.1016/j.ydbio.2011.02.008.
Gehring WJ: The master control gene for morphogenesis and evolution of the eye. Genes Cells. 1996, 1: 11-15. 10.1046/j.1365-2443.1996.11011.x.
Shaham O, Menuchin Y, Farhy C, Ashery-Padan R: Pax6: a multi-level regulator of ocular development. Prog Retin Eye Res. 2012, 31: 351-376. 10.1016/j.preteyeres.2012.04.002.
Tsonis PA, Fuentes EJ: Focus on molecules: Pax-6, the eye master. Exp Eye Res. 2006, 83: 233-234. 10.1016/j.exer.2005.11.019.
Lakowski J, Majumder A, Lauderdale JD: Mechanisms controlling Pax6 isoform expression in the retina have been conserved between teleosts and mammals. Dev Biol. 2007, 307: 498-520. 10.1016/j.ydbio.2007.04.015.
Zhang W, Cveklova K, Oppermann B, Kantorow M, Cvekl A: Quantitation of PAX6 and PAX6(5a) transcript levels in adult human lens, cornea, and monkey retina. Mol Vis. 2001, 7: 1-5.
Kim J, Lauderdale JD: Analysis of Pax6 expression using a BAC transgene reveals the presence of a paired-less isoform of Pax6 in the eye and olfactory bulb. Dev Biol. 2006, 292: 486-505. 10.1016/j.ydbio.2005.12.041.
Kiselev Y, Eriksen TE, Forsdahl S, Nguyen LH, Mikkola I: 3 T3 cell lines stably expressing Pax6 or Pax6(5a)–a new tool used for identification of common and isoform specific target genes. PLoS One. 2012, 7: e31915-10.1371/journal.pone.0031915.
Edqvist PH, Myers SM, Hallbook F: Early identification of retinal subtypes in the developing, pre-laminated chick retina using the transcription factors Prox1, Lim1, Ap2alpha, Pax6, Isl1, Isl2, Lim3 and Chx10. Eur J Histochem. 2006, 50: 147-154.
Kuriyama F, Ueda Y, Araki M: Complete reconstruction of the retinal laminar structure from a cultured retinal pigment epithelium is triggered by altered tissue interaction and promoted by overlaid extracellular matrices. Dev Neurobiol. 2009, 69: 950-958. 10.1002/dneu.20745.
Nabeshima A, Nishibayashi C, Ueda Y, Ogino H, Araki M: Loss of cell-extracellular matrix interaction triggers retinal regeneration accompanied by Rax and Pax6 activation. Genesis. 2013, 51: 410-419. 10.1002/dvg.22378.
Thummel R, Enright JM, Kassen SC, Montgomery JE, Bailey TJ, Hyde DR: Pax6a and Pax6b are required at different points in neuronal progenitor cell proliferation during zebrafish photoreceptor regeneration. Exp Eye Res. 2010, 90: 572-582. 10.1016/j.exer.2010.02.001.
Haubst N, Berger J, Radjendirane V, Graw J, Favor J, Saunders GF, Stoykova A, Gotz M: Molecular dissection of Pax6 function: the specific roles of the paired domain and homeodomain in brain development. Development. 2004, 131: 6131-6140. 10.1242/dev.01524.
Berger J, Berger S, Tuoc TC, D'Amelio M, Cecconi F, Gorski JA, Jones KR, Gruss P, Stoykova A: Conditional activation of Pax6 in the developing cortex of transgenic mice causes progenitor apoptosis. Development. 2007, 134: 1311-1322. 10.1242/dev.02809.
Nagashima M, Barthel LK, Raymond PA: A self-renewing division of zebrafish Muller glial cells generates neuronal progenitors that require N-cadherin to regenerate retinal neurons. Development. 2013, 140: 4510-4521. 10.1242/dev.090738.
Nelson CM, Ackerman KM, O'Hayer P, Bailey TJ, Gorsuch RA, Hyde DR: Tumor necrosis factor-alpha is produced by dying retinal neurons and is required for Muller glia proliferation during zebrafish retinal regeneration. J Neurosci. 2013, 33: 6524-6539. 10.1523/JNEUROSCI.3838-12.2013.
Haynes T, Luz-Madrigal A, Reis ES, Echeverri Ruiz NP, Grajales-Esquivel E, Tzekou A, Tsonis PA, Lambris JD, Del Rio-Tsonis K: Complement anaphylatoxin C3a is a potent inducer of embryonic chick retina regeneration. Nat Commun. 2013, 4: 2312-
Cimadamore F, Amador-Arjona A, Chen C, Huang CT, Terskikh AV: SOX2-LIN28/let-7 pathway regulates proliferation and neurogenesis in neural precursors. Proc Natl Acad Sci U S A. 2013, 110: E3017-E3026. 10.1073/pnas.1220176110.
Primer3web version 4.0.0. [http://primer3.wi.mit.edu/]
Bustin SA, Benes V, Garson JA, Hellemans J, Huggett J, Kubista M, Mueller R, Nolan T, Pfaffl MW, Shipley GL, Vandesompele J, Wittwer CT: The MIQE guidelines: minimum information for publication of quantitative real-time PCR experiments. Clin Chem. 2009, 55: 611-622. 10.1373/clinchem.2008.112797.
Schmittgen TD, Livak KJ: Analyzing real-time PCR data by the comparative C(T) method. Nat Protoc. 2008, 3: 1101-1108. 10.1038/nprot.2008.73.
Image J. Image Processing and Analysis in Java. [http://rsb.info.nih.gov/ij/]
Dr R Edelmann and the Microscopy Facility at Miami University; Dr A Kiss from The Center for Bioinformatics and Functional Genomics (CBFG) at Miami University; M Hughes from the Department of Statistics for his expertise on statistical analyses; C Closson and Dr Y Zavros from the Department of Molecular and Cellular Physiology at the University of Cincinnati for facilitating the use of the laser capture microdissection system; J Dannenfelser for her various technical contributions to this work. This work was supported by EY17319 to KDRT, EY10540 to PAT, and CONACYT 162930 and 142523 to AL-M. The Zeiss confocal microscope is supported by an NSF-MRI award DBI-0821211.
The authors declare that they have no competing interests.
AL-M designed and performed experiments, analyzed data and co-wrote the paper. EG-E, AM, AMD and KB-S performed experiments and analyzed data. PAT discussed experiments, analyzed data and co-wrote the paper. KDRT conceived the idea, supervised the work, designed experiments, analyzed the data and co-wrote the paper. All authors have read and approved the final manuscript.