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Nolz1 is a zinc finger transcription factor whose expression is enriched in the lateral ganglionic eminence (LGE), although its function is still unknown.
Here we analyze the role of Nolz1 during LGE development. We show that Nolz1 expression is high in proliferating neural progenitor cells (NPCs) of the LGE subventricular zone. In addition, low levels of Nolz1 are detected in the mantle zone, as well as in the adult striatum. Similarly, Nolz1 is highly expressed in proliferating LGE-derived NPC cultures, but its levels rapidly decrease upon cell differentiation, pointing to a role of Nolz1 in the control of NPC proliferation and/or differentiation. In agreement with this hypothesis, we find that Nolz1 over-expression promotes cell cycle exit of NPCs in neurosphere cultures and negatively regulates proliferation in telencephalic organotypic cultures. Within LGE primary cultures, Nolz1 over-expression promotes the acquisition of a neuronal phenotype, since it increases the number of β-III tubulin (Tuj1)- and microtubule-associated protein (MAP)2-positive neurons, and inhibits astrocyte generation and/or differentiation. Retinoic acid (RA) is one of the most important morphogens involved in striatal neurogenesis, and regulates Nolz1 expression in different systems. Here we show that Nolz1 also responds to this morphogen in E12.5 LGE-derived cell cultures. However, Nolz1 expression is not regulated by RA in E14.5 LGE-derived cell cultures, nor is it affected during LGE development in mouse models that present decreased RA levels. Interestingly, we find that Gsx2, which is necessary for normal RA signaling during LGE development, is also required for Nolz1 expression, which is lost in Gsx2 knockout mice. These findings suggest that Nolz1 might act downstream of Gsx2 to regulate RA-induced neurogenesis. Keeping with this hypothesis, we show that Nolz1 induces the selective expression of the RA receptor (RAR)β without altering RARα or RARγ. In addition, Nozl1 over-expression increases RA signaling since it stimulates the RA response element. This RA signaling is essential for Nolz1-induced neurogenesis, which is impaired in a RA-free environment or in the presence of a RAR inverse agonist. It has been proposed that Drosophila Gsx2 and Nolz1 homologues could cooperate with the transcriptional co-repressors Groucho-TLE to regulate cell proliferation. In agreement with this view, we show that Nolz1 could act in collaboration with TLE-4, as they are expressed at the same time in NPC cultures and during mouse development.
Nolz1 promotes RA signaling in the LGE, contributing to the striatal neurogenesis during development.
During the first stages of striatal development, neurons arise from the ventricular zone (VZ), which is mainly composed of neuroepithelial cells [1,2]. Around embryonic day (E)11.5, these cells divide asymmetrically; giving rise to radial glial cells and neural progenitor cells (NPCs). Radial glial cells have extensions that contact with the ventricular lumen and with more differentiated inner zones of the developing striatum, but their cell bodies remain in the VZ [3-5]. In contrast, NPCs leave the VZ to proliferate and generate the so-called subventricular zone (SVZ). Within the dorsal telencephalon, the SVZ is a thin layer of cells, mainly formed of NPCs [4,6]. However, in the ventral telencephalon, it becomes a prominent structure that has been shown to be the main source of striatal neurons and glia. Striatal projecting neurons are born in the SVZ of the lateral ganglionic eminence (LGE) whereas the medial ganglionic eminence will give rise to cortical and striatal interneurons.
Retinoic acid (RA) is one of the morphogens that participates in the specification and differentiation of the intermediate position of the LGE in the telencephalon . However, RA sources during telencephalon development are still unclear. Three different retinaldehyde dehydrogenases (Raldhs), the limiting enzymes for RA synthesis, have been described in the central nervous system. Two of them, Raldh2 and Raldh3, are expressed in the otic vesicles and frontonasal ectoderm, respectively, as early as E8.5 [8-10]. Thus, it is unlikely that RA from these sources could reach the intermediate telencephalon. Around E12.5, Raldh3 expression appears in the LGE, providing the first known source of RA in the striatum [9,11]. During this period, the expression of the RA receptors (RARs) RARα and RARβ is high in the ventral telencephalon and it has been shown that RARβ stimulation mediates gene regulation in the developing telencephalon, particularly on striatal neuronal populations  where 95% of neurons are GABAergic . In addition, RA increases the number of GABAergic neurons in differentiating mouse embryonic stem cells through the regulation of RARβ [14,15]. Some transcription factors are of great importance for RA signaling in the LGE. Among these is the homeobox transcription factor Gsx2, which is essential for correct striatal development [16,17] and for Raldh3 expression. Raldh3 levels are severely reduced or lost in mice deficient for Gsx2 or Gsx1 and Gsx2 .
To exert its effect during development, RA binds specific RARs and, thereafter, regulates the expression of some transcription factors that contain a RA response element (RARE) in their promoter. One of these transcription factors is Nolz1, which is induced by RA in the PC12 neural cell line and during developing chick spinal cord [19,20]. Nolz1 is a member of the NocA-Elbow (elB)-Tlp (NET) family of transcription factors, which are involved in patterning and differentiation during development in all studied species [21-24]. In zebrafish, two members of the NET family have been identified, nlz1 and nlz2, and both have been described to be essential for boundary formation in the rombencephalon [23,24]. Nlz2 is also expressed in more anterior structures, including the telencephalic vesicles, where it is supposed to play similar roles in regionalization . A Nlz2 homolog in rodents was called Nolz1 (also known as Zfp503), which is expressed during nervous system development in several regions, including the hypothalamus and spinal cord. However, its highest expression is localized in the ventral LGE (vLGE) [19,26]. Of note, Nolz1 is totally absent in close telencephalic structures such as the medial ganglionic eminence and the pallidum, including the dorsal LGE (dLGE) , suggesting a highly specific striatal function. However, this family of transcription factors cannot directly interact with DNA, indicating that they need to interact with other transcription factors. In Drosophila, it has been shown that elbow B (elB) interacts with Groucho (Gro) proteins, forming large complexes of proteins that act as transcriptional co-repressors .
Despite its characterized pattern of expression, the function of Nolz1 during telencephalic development has not been analyzed yet. Here we studied the role of Nolz1 during vLGE development and the relationship between Nolz1 and the RA pathway within the LGE. Our results show that Nolz1 induces cell cycle exit and promotes neuronal differentiation. In addition, we also demonstrate that Nolz1 expression is temporarily regulated by RA during early striatal development. Finally, we show that Nolz1 contributes to neuronal differentiation through the increase of RA signaling.
In order to analyze whether the temporal expression pattern of Nolz1 protein resembles that of Nolz1 mRNA, a polyclonal antibody was raised against 12 amino acids of the amino terminus of the Nolz1 protein sequence (Figure (Figure1A).1A). Western blotting of NPC lysates showed that the antibody recognizes a unique specific band when compared to the pre-serum blotted membrane (Figure (Figure1B).1B). In addition, dot blot analyses demonstrated the specificity of the serum (Figure (Figure1C),1C), which could be blocked by the competitive incubation of the antibody with the Nolz1 peptide (Figure (Figure1D).1D). Using this Nolz1 polyclonal antibody, we performed western blot analysis in striatal samples from E14.5, E18.5, postnatal day (P)3 and adult mice. Our results showed that Nolz1 levels are high at embryonic stages, being down-regulated postnatally (Figure (Figure2A).2A). Within the adult, low levels of Nolz1 protein remained in the striatum while no expression was detected in the subependymal zone (Figure (Figure2A).2A). In situ hybridization for Nolz1 showed high levels of mRNA in the SVZ of the vLGE at E14.5 (Figure (Figure2B).2B). No signal was detected in the dLGE (Figure (Figure2B),2B), which gives rise to olfactory bulb interneurons during development . Low levels of Nolz1 mRNA were also detected in the mantle zone (MZ; Figure 2B,D), where it partially co-localized with Tuj1-positive neurons (Figure 2D,E). In the adult brain, similar to the protein results, Nolz1 mRNA was not detected in the subependymal zone, although faint expression could still be detected in the striatum by in situ hybridization (Figure (Figure2C2C).
The high levels of Nolz1 expression in the SVZ of the vLGE suggest it has a role in the regulation of NPC homeostasis. Thus, to analyze the function of Nolz1 in NPCs, we generated neurospheres from the LGE of E14.5 mice. Nolz1 expression was analyzed in proliferating cells and at 3 and 6 days in vitro (DIV) after the induction of neurosphere differentiation (Figure 3A,B). We observed that Nolz1 expression levels were high in non-differentiated cells, while its expression decreased during the differentiation process for both mRNA (Figure (Figure3A)3A) and protein (Figure (Figure3B).3B). These results were coincident with the expression pattern of Nolz1 in vivo, which mainly corresponded to the NPC-containing SVZ (Figure (Figure2B2B).
We next analyzed whether Nolz1 regulates NPC proliferation. Over-expression of human Nolz (hNolz) in NPCs led to high hNolz mRNA levels but a significant decrease in endogenous mouse Nolz1 expression (Figure (Figure4A),4A), suggesting tight regulation of mouse Nolz1 levels. When we analyzed Nolz protein levels with a Nolz1 antibody that detects mouse and human isoforms, we found a net increase in Nolz protein levels with respect to control transfected cells (Figure (Figure4B).4B). hNolz-over-expressing neurospheres showed a 19.5% reduction in the number of proliferating bromodeoxyuridine (BrdU)-positive NPCs with respect to control transfected cells (Figure 4D,E). Double immunocytochemistry showed that most, but not all, of the hNolz-over-expressing cells were negative for BrdU (Figure (Figure4D).4D). To verify that the reduction in BrdU-positive cells was due to cell cycle exit and not to variations in its duration, we measured the cell cycle time of transfected NPCs as described elsewhere  and did not find any difference between control and hNolz-over-expressing neurospheres (DsRED, 25.29 h; hNolz-DsRED, 24.88 h). In addition, we analyzed the index of cell cycle exit as described previously by Chenn and Walsh . This demonstrated that hNolz over-expression produces a significant increase of 162% in the cell cycle exit index (Figure (Figure4G).4G). Since the reduction in the number of BrdU-positive NPCs may also be due to cell death, we also counted the number of apoptotic nuclei of hNolz-over-expressing NPCs with respect to control enhanced green fluorescent protein (EGFP)-transfected NPCs. No cell death was observed in any condition (data not shown).
In addition, the effect of Nolz1 silencing was also analyzed by using a cocktail of three different Nolz1 small interfering RNAs (siRNAs) at a concentration of 2 μM, which led to 60% inhibition of Nolz1 mRNA (data not shown) and 82% inhibition of Nolz1 protein expression 2 DIV after transfection (Figure (Figure4C).4C). As expected, transfection of Nolz1 siRNA increased the number of BrdU-positive NPCs (by 18.5%) in the neurosphere cultures with respect to scrambled negative siRNA control transfection (Figure (Figure4E).4E). Taken together, these findings demonstrate that deregulation of Nolz1 altered the proliferating capacity of NPCs, suggesting that Nolz1 promotes cell cycle exit. Next, we studied the capacity of NPCs to form new neurospheres 5 DIV after hNolz over-expression or transfection of Nolz1 siRNA (Figure (Figure4F).4F). hNolz negatively regulated NPC self-renewal, as shown by the decrease in the number of new neurospheres formed after hNolz over-expression and the corresponding increase observed after Nolz1 siRNA transfection (Figure (Figure4E,4E, P0). When cells were dissociated and plated again (P1), no differences were observed in any condition studied (Figure (Figure4E).4E). These findings indicate a transient effect of Nolz1 and that variation of the levels of this transcription factor does not permanently affect NPC populations since hNolz over-expression or Nolz1 siRNA was lost after the first passage.
To further confirm the role of Nolz1 in the regulation of NPC proliferation, we next electroporated hNolz into LGE-derived organotypic cultures from E15.5 embryos and analyzed the number of Ki67-positive cells (Figure (Figure5).5). Two days after electroporation, hNolz over-expression reduced the proliferation of NPCs at the SVZ as indicated by the dramatic decrease in the number of Ki67-positive cells with respect to the control electroporated side (Figure (Figure5B5B).
Reduced proliferation of NPCs could be indicative of neural differentiation. To test this possibility, we first analyzed whether Nolz1 was expressed in differentiated post-mitotic cells in primary cultures derived from E14.5 LGEs (Figure 6A,B). Double immunocytochemistry against Nolz1 and the neural markers Tuj1 or glial fibrillary acidic protein (GFAP) showed that most of the Nolz1-positive cells were positive for the neuronal marker Tuj1, while we could not find any overlap between Nolz1 and the astroglial marker GFAP (Figure 6A,B). We also analyzed the role of Nolz1 on neural differentiation by transfecting LGE primary cultures with plasmids that express hNolz-EGFP or EGFP alone as control (Figure 6C,D). Five days after transfection, we performed double immunocytochemistry for GFP and the neural precursor gene nestin, the neuronal markers Tuj1 and microtubule-associated protein (MAP)2 or the astroglial marker GFAP. hNolz-over-expressing cells mainly colocalized with the neuronal markers Tuj1 and MAP2, although some double GFP-nestin stained cells were also observed (Figure (Figure6C).6C). In contrast, no astroglial cell markers were seen in hNolz transfected cells, as shown by the lack of colocalization between GFP and GFAP (Figure (Figure6C).6C). Interestingly, the quantification of the double positive cells in hNolz (hNolz-EGFP) versus control transfected cells (EGFP) demonstrated that hNolz promotes a neuronal phenotype (Figure (Figure6D).6D). hNolz over-expression increased the number of both Tuj1- and MAP2-positive neurons, which was accompanied by a reduction in the number of nestin-positive cells (Figure (Figure6D).6D). In addition, no hNolz-over-expressing cells were GFAP-positive astroglia (Figure (Figure6D6D).
To determine whether RA is needed for Nolz1 expression in striatal cells during development, pregnant mice were fed with a vitamin A (retinol)-deficient diet, which results in a general decrease of RA blood levels . In these animals the levels of RARβ were partially reduced (Figure (Figure7A),7A), indicating a decrease in RA levels since it is well known that this receptor is regulated by RA signals. Analysis of Nolz1 expression in E14.5 embryos developed under these vitamin A-deficient levels did not show any difference with respect to expression in regular fed wild-type control embryos (Figure 7B,C). To further confirm that the lack of RA does not affect Nolz1 expression, we analyzed the levels of Nolz1 expression in Raldh3-/- embryos (Figure (Figure7D),7D), which have completely lost RA activity . Nolz1 expression was not affected by the absence of Raldh3 in the LGE at E14.5 (Figure (Figure7D),7D), further corroborating the independence of Nolz1 expression from RA signaling in the vLGE at this developmental stage.
To analyze whether Nolz1 expression levels were regulated by RA in vitro, LGE-derived neurospheres were treated with increasing concentrations of RA during 3 DIV and the levels of Nolz1 were analyzed by quantitative PCR (Q-PCR). Nolz1 expression was increased by RA in E12.5-derived NPC cultures (Figure (Figure8A).8A). However, it was not affected in E14.5-derived NPC cultures (Figure (Figure8C).8C). As a well known RA-induced control gene, we analyzed RARβ, which was clearly upregulated in a dose-dependent manner at both stages (Figure 8B,D). Coincidentally, Nolz1 expression did not change in E14.5 LGE primary cultures treated with RA, although RARβ was also increased in these cultures (Figure (Figure8E).8E). Therefore, striatal cultures were competent to increase Nolz1 expression in response to RA treatment at E12.5 but not at later stages. In agreement with these results, when we treated mouse embryonic stem cells with RA, Nolz1 expression was upregulated in a dose-dependent manner (Figure (Figure9),9), supporting that Nolz1 competence to RA signaling depends on early developmental stages.
Since Gsx2 is essential for the correct expression of several RA-dependent genes, such as Raldh3, in the LGE , we also examined the expression of Nolz1 in Gsx2 knockout mice. Nolz1 expression was analyzed by in situ hybridization in knockout mice carrying a single (Gsx2+/EGFP) or double substitution of the Gsx2 gene for EGFP (Gsx2EGFP/EGFP) . Low levels of Nolz1 expression remained in the Gsx2 heterozygous mouse vLGE at E14.5 (Figure 10A,B), but no signal was detected in the Gsx2EGFP/EGFP mice (Figure 10C), indicating that Gsx2 is critical for Nolz1 expression. On the other hand, over-expression of Gsx2 in NPCs did not lead to an increase in Nolz1 mRNA levels, while it enhanced the levels of Raldh3 mRNA (Figure 10D), which has been shown to be regulated by Gsx2 . These findings indicate that Gsx2 is essential but not sufficient to induce Nolz1 expression.
The specific combination of RA receptors defines the competence of cells to respond to RA. Thus, we next analyzed whether Nolz1 expression regulates RARs. We measured RARα, RARβ and RARγ mRNA levels 2 and 5 DIV after hNolz over-expression or silencing with Nolz1 siRNA in NPCs (Figure 11A). We did not detect RARγ expression in control NPCs, or after transfection of hNolz or Nolz1 siRNA (data not shown). In contrast, both RARα and RARβ were highly expressed in NPCs. RARα levels were not modified in any condition studied whereas RARβ levels were increased 5 DIV after hNolz over-expression and reduced after Nolz1 silencing (Figure 11A). In addition, hNolz over-expression did not regulate the level of Raldh3 mRNA (Figure 11A). Similarly, the levels of CRBP1 and Cyp26, two other limiting proteins for RA metabolism, were not modified by hNolz overexpression (data not shown). These findings indicate that Nolz1 expression does not increase RA levels but changes the competence of cells to respond to RA. To further test this hypothesis, we analyzed whether hNolz over-expression could activate RA signaling using a Luciferase RARE-reporter assay. Three DIV after transfection, an increase in luciferase activity was observed (Figure 11B), demonstrating that this transcription factor leads to an increase in RA signaling. These results suggested that Nolz1 could induce the conversion of NPCs into neuronal cells through the regulation of RARβ-mediated signaling. Thus, we next analyzed whether Nolz1 mediates NPC cell cycle exit and promotes neuronal differentiation by this mechanism. Surprisingly, RA signaling does not seem to mediate Nolz1-regulated proliferation of NPCs, since under the same conditions that hNolz modified BrdU incorporation, treatment with RA (Figure 12A) or a RARβ-specific agonist (Figure 12B) did not affect neurosphere proliferation (Figure (Figure12).12). Thus, we next analyzed whether RA signaling was necessary for Nolz1-induced neurogenesis. To this end, we transfected primary striatal cultures with hNolz in the absence of RA, since cells were cultured in a RA-free medium supplemented with 4-diethylaminobenzaldehyde (DEAB), a Raldh inhibitor . Under these conditions, the levels of RARβ and Raldh3 were highly reduced (Figure 13A). Moreover, hNolz could not induce neuronal differentiation in the absence of RA, since hNolz-induced neurogenesis was lost in the presence of DEAB (Figure 13B,C). To further study whether the effect of Nolz1 in neurogenesis was not only dependent on RA but also on RARβ signaling, we next over-expressed hNolz in striatal primary cultures treated with a pan-RAR inverse agonist (BMS493, also named UVI2024, [34,35]). In these conditions, hNolz was also unable to induce an increase of Tuj1-positive cells and a reduction of nestin-positive precursors or GFAP-positive astroglia (Figure (Figure14).14). Therefore, these results demonstrate that Nolz1 needs RA signaling through RARs to mediate striatal neurogenesis. However, the stimulation of RARβ with a specific agonist (BMS641, also named UVI2003, ) was not sufficient to induce changes in neural markers in striatal cultures (Figure (Figure1515).
Due to the ability of the NET family of transcription factors, which includes Nolz1, to bind to members of the Gro-TLE family of transcriptional repressors [22,20,24], we analyzed the expression of several members of the Gro-TLE family in the LGE at E14.5 by in situ hybridization (Figure (Figure16).16). We did not detect any Tle2 expression, and Tle3 mRNA was slightly but broadly expressed through the telencephalon (Figure 16A). Tle1 and Tle4, in contrast, were specifically regulated in the different proliferative zones of the LGE (Figure 16A). Tle1 expression was maximal in the VZ, and decreased in the SVZ and MZ (Figure 16A). In contrast, Tle4 was not expressed in the VZ and its levels were high in the SVZ, extending to the MZ but at lower expression levels (Figure 16A), thus resembling the expression pattern of Nolz1 (Figure (Figure2).2). To determine if Nolz1 and Tle4 were co-expressed in the LGE, we performed in situ hybridization for Nolz1 followed by immunohistochemistry for Tle4, which confirmed their colocalization within the LGE (Figure 16B). We also analyzed the Tle4 expression pattern during NPC differentiation. Tle4 followed a pattern of expression similar to that of Nolz1, as its maximal levels were achieved in non-differentiated NPCs and decreased with differentiation (Figure 16C).
Our results show that Nolz1 expression is high in the SVZ and is maintained at low levels in the MZ of the LGE, suggesting a dual effect promoting cell cycle exit and neuronal differentiation of NPCs. We found that Nolz1 expression negatively regulates the proliferation and induces cell cycle exit of NPCs cultured as neurospheres. In addition, in LGE-derived primary neural cultures, Nolz1 over-expression increased the number of neurons at the expense of nestin- and GFAP-positive cells, indicating that Nolz1 participates in striatal neurogenesis. We also show that Nolz1-induced neurogenesis depends on RA signaling, since this transcription factor promoted the expression of RARβ in LGE-derived NPCs and its neurogenic effect was impaired in a RA-signaling-free context.
The shape of the telencephalon and the relative sizes and positions of its cell populations result from variations in cell proliferation  and many transcription factors have important roles in this mechanism. Our results show that Nolz1 contributes to the homeostasis of NPCs in the SVZ of the vLGE, where it is highly expressed ( and our present results), by reducing the proliferation, promoting cell cycle exit and possibly reducing the self-renewal potential of NPCs. Cell cycle exit during LGE embryonic development is usually associated with proneural transcription factors. Here we demonstrate that Nolz1 promotes the acquisition of a neuronal phenotype since over-expression of Nolz1 in LGE primary cultures produces an increase in the number of neurons. Proneural factors such as Ascl I (also known as Mash1)  are restricted to the VZ and SVZ, where progenitors begin to differentiate, but are absent in the MZ, where fully differentiated neurons are found. However, other transcription factors such as Meis2 or Islet are expressed in both the germinal VZ and SVZ and in the MZ [28,38]. Similarly, Nolz1 expression is high in the SVZ and its expression decreases but does not disappear in the MZ, where striatal neurons continue to express low levels of Nolz1 ( and present results). These results agree with the idea that stable specification of cell identity requires mechanisms that maintain patterns of gene expression over long periods of time .
One of the main issues in cell fate specification is the understanding of the interaction between two general sets of determinative factors: secreted extrinsic signals present in a cell's local environment and intrinsic signals that operate in a cell-autonomous manner . Keeping with this view, RA signaling can increase Nolz1 levels in the PC12 cell line  and in chick postmitotic motoneurons . Our results demonstrate that Nolz1 expression was not modified when a vitamin A-deficient diet was used to feed the mothers, which results in lowered levels of RA synthesis in the pups throughout the whole of development . In addition, Nolz1 expression was not affected in Raldh3-deficient animals, which have been shown to lack RA activity in the LGE . These findings suggest that the levels of RA are not limiting for Nolz1 expression. Reinforcing this idea, we observed that RA does not regulate Nolz1 expression in E14.5-derived NPCs or primary cultures. However, E12.5-derived NPCs do respond to RA by increasing the expression of Nolz1. Similarly, RA was able to regulate Nolz1 in mouse embryonic stem cells. Altogether, these data indicate that the ability of cells to induce Nolz1 in response to RA is dynamically regulated during striatal development. Thus, a very interesting possibility is that RA participates in the induction but not in the maintenance of Nolz1 expression, since other sources of RA in the LGE has been described .
Interestingly, we found that Gsx2 is required for the correct expression of Nolz1 in the vLGE, the mouse telencephalic structure that gives rise to striatal projection neurons (for a review, see ). In agreement with this result, it has recently been shown that Gsx2 participates in the temporal specification of neuronal fate in the LGE . The development of striatal projection neurons depends on early actions of Gsx2 during differentiation of the vLGE, where Nolz1 is expressed, while differentiation of the dLGE, where Nolz1 is not expressed, requires Gsx2 function at least until birth . However, over-expression of Gsx2 in NPCs did not modify the levels of Nolz1, suggesting that Gsx2 acts as a permissive instead of an inductive factor for Nolz1 expression. Since Gsx2 is involved in the differentiation of striatal projecting neurons through the regulation of RA signaling , Nolz1 could act downstream of Gsx2 to regulate RA signaling. We found that Nolz1 regulates the expression of RARβ, the RA receptor that has been shown to promote striatal projection neuron differentiation [12,15,43]. In addition, early striatal neurogenesis is affected in RARβ mutant mice , coinciding with the expression and function of Nolz1. In fact, Nolz1 and RARβ are expressed in the MZ at the same developmental stages ([19,45] and present results). Furthermore, our present results demonstrate that Nolz1 induces not only increases in RARβ but also RA signaling, which is essential to exert its neurogenic effect in primary striatal cultures. Interestingly, although this receptor is necessary for Nolz1-induced neurogenesis, its activation by a selective RARβ agonist is not sufficient to stimulate any changes in neural markers. This result suggests that Nolz1 may also act on additional pathways to promote neural differentiation. Altogether, these findings show that Nolz1 participates in the early Gsx2-dependent differentiation of vLGE-derived neurons through the regulation of RARβ-mediated signaling.
It has been shown that Gsx2 mutant mice have reduced levels of Raldh3 . In addition, we show that over-expression of Gsx2 in NPCs increases the mRNA levels of this striatal RA-limiting enzyme. However, we observed that Nolz1 did not regulate the expression of Raldh3, so it is not regulating RA synthesis. These results suggest that Gsx2 may regulate RA signaling at two different levels; one is Nolz-independent and mediated by the regulation of Raldh3 and the other involves the regulation of Nolz1 expression, which in turn regulates the levels of RARβ.
RARβ is expressed in the MZ while RARα is broadly expressed in the VZ and SVZ through the entire telencephalon and is important in the control of the proliferation of neural precursors [11,46]. We observed that RARα is unaffected by Nolz1 over-expression. Thus, it seems that Nolz1 acts through RA signaling to regulate the differentiation of striatal projection neurons but its effect on NPC proliferation is independent of RA. In fact, we observed that RA did not modify the proliferation of NPCs in vitro. Increases in cell cycle length could lead to progressive restriction of the proliferation potential of LGE NPCs, and it can be promoted by transcription factors such as Foxg1 . However, Nolz1 did not induce changes in cell cycle length. Another interesting possibility is that Nolz1 and Gsx2 function together to regulate proliferation since Gsx2 expression in the SVZ coincides with Nolz1 ([19,32] and present results). Keeping with this view, it has been shown that the Gsx2 homolog in Drosophila, Ind (intermediate neuroblasts defective), interacts with Gro proteins, which are able to bind elB (elbow B), the Nolz1 homolog, acting as transcriptional co-repressors . In addition, the mammalian Nolz1 protein also contains the conserved FKPY sequence, which allows binding to Gro-TLE proteins (Figure (Figure1A).1A). We observed that many TLE (NocA-elB-Tlp) proteins, the mammalian homologs of Gro, are expressed in the vLGE. Among them, TLE4 follows a similar expression pattern to Nolz1, with its highest levels in the SVZ, while the VZ is enriched in TLE1 expression. These results are similar to those observed in the cerebral cortex, where TLE4 is expressed by more differentiated NPCs of the SVZ and TLE1 expression is elevated in the undifferentiated VZ neural precursors [47-49]. Moreover, TLE4 expression decreased upon NPC differentiation. Taken together, these findings suggest that Nolz1 and TLE4 could act together to control SVZ proliferation in the LGE. Similarly, it has been recently described that Nolz1 requires, in part, the modulatory activity of Grg5, an atypical member of the Gro-TLE family of co-repressors, to control motor neuron determination in the chick spinal cord . However, further experiments are required to analyze functional interactions between these proteins.
In conclusion, we demonstrate that Nolz1 has a dual effect on NPCs, on one hand by controlling their proliferation and promoting cell cycle exit, and on the other by inducing striatal neurogenesis. Nolz1 over-expression increases the number of striatal neurons downstream of Gsx2 by inducing RA signaling through RARs. Its properties and expression pattern suggest that the activity of Nolz1 in the vLGE could be modulated by co-repressors, such as Gro-TLE.
All animals were housed with access to food and water ad libitum in a colony room maintained at a constant temperature (19 to 22°C) and humidity (40 to 50%) on a 12:12 h light:dark cycle. Animal treatments and handling procedures were approved by the Local Committees, in accordance with the European Community Council Directive (86/609/EU).
B6CBA wild-type mice (from Charles River Laboratories, Les Oncins, France), Raldh3-deficient mice , and Gsx2-deficient mice  were used in this study. For embryonic ages, time of pregnancy was determined by first detection of a vaginal sperm plug by daily inspection and considered as E0.5. For postnatal studies, the day of birth was considered as postnatal day 0 (P0).
To induce vitamin A deficiency in mice, pregnant mice were fed with the vitamin A-deficient diet TD.86143 (Harlan Laboratories Inc., Indianapolis, IN, USA).
E12.5 or E14.5 fetal brains were excised and placed in sterile phosphate-buffered saline pH 7.4, and the LGEs were dissected bilaterally, pooled and gently dissociated with a fire-polished Pasteur pipette.
Mixed neuron-glial primary cultures were obtained by plating the cells onto 24-well plates containing glass coverslips precoated with 0.1 mg/ml poly-D-lysine (Sigma Chemical Co., St Louis, MO, USA) at a density of 150,000 cells/cm2 in Eagle's minimum essential medium (Invitrogen SA, Prat de Llobregat, Barcelona, Spain) supplemented with 7.5% fetal bovine serum (FBS; Invitrogen SA), 0.6% D-(+)-glucose (Sigma Chemical Co.), 100 U/mL of penicillin and 100 mg/mL streptomycin (both obtained from Invitrogen SA). Three or 5 days after seeding, cultures were fixed with 4% paraformaldehyde solution (PFA; Merck Biosciences Ltd, Nottingham, UK) in 0.1 M phosphate buffer pH 7.4 and processed for immunocytochemistry.
LGE-derived neurosphere cultures were obtained by seeding 50,000 cells/cm2 in medium containing Dubelcco's Modified Eagle's Medium (DMEM; Sigma Chemical Co.):F12 (Invitrogen SA) (1:1); supplemented with 0.3% glucose (Sigma Chemical Co.), 0.3 mg/ml glutamine (Invitrogen SA), 5 mM HEPES (Invitrogen SA), 100 U/ml penicillin, and 100 mg/ml streptomycin (Invitrogen SA), 4 μg/ml heparin (Sigma Chemical Co.), 4 mg/ml bovine serum albumin (Sigma Chemical Co.), 1× N2 supplement (Invitrogen SA), 20 ng/ml fibroblast growth factor (Sigma Chemical Co.) and 10 ng/ml epidermal growth factor (Invitrogen SA). Every 5 days neurospheres were collected, dissociated by pipetting approximately 40 times with a P100 micropipette and re-plated in fresh media at a density of 10,000 cells/cm2.
For cell differentiation, 12,500 cells/cm2 were seeded. The day after plating, cells were collected and incubated onto Matrigel-treated coverslips (Growth Factor Reduced Matrigel Matrix, BD Biosciences, Clontech-Takara Bio Europe, Saint-Germain-en-Laye, France). Media was changed to medium supplemented with only 20 ng/ml fibroblast growth factor (Sigma Chemical Co.) and cells were allowed to differentiate in this medium for 2 more days. Then, media was changed again to medium supplemented with 2% FBS (Invitrogen SA) and cells were grown for 3 more days (until a total of 6 days of in vitro differentiation). Cell pellets for each time point (0, 3 and 6 days of differentiation) were obtained and frozen at -80°C for RNA or protein extraction.
In the present study, we used the mouse embryonic stem cell line R1 obtained from Dr Andras Nagy's laboratory. The maintenance of undifferentiated mouse embryonic stemcells, embryoid body formation and culture were carried out as previously described .
All cell cultures were incubated at 37°C in a 5% CO2 atmosphere.
Neurospheres were passaged as described above and single cells were seeded in 6-well plates at a density of 100 cells/mm2 with fresh culture medium containing different concentrations of all-trans-RA (10-9, 10-8 and 10-6 M; Sigma Chemical Co.) dissolved in dimethyl sulfoxide (DMSO; Sigma Chemical Co.). Control cells were cultured with the same dilutions of the RA vehicle, DMSO. Some cultures were treated with a RARβ-specific agonist  at a concentration of 10-8 M dissolved in DMSO, which we observed is effective in these cultures (R Martín-Ibáñez et al., in preparation). NPCs were allowed to grow for 3 DIV and then were pelleted for RNA extraction and RT-PCR analysis or processed for BrdU immunocytochemistry.
Mixed neuron-glial LGE primary cultures were grown for 3 DIV and RA or RARβ agonist (BMS641) dissolved in DMSO was added to the medium at the concentration of 10-8 M. Fresh RA/RARβ agonist was added every 24 hours of culture and 3 hours prior to fixation.
Embryoid bodies were formed as described above and RA was added to the culture medium at different concentrations (10-9, 10-8 and 10-6 M). They were grown for 4 DIV and then pelleted for RNA extraction and RT-PCR analysis.
To over-express NolzI, cells were transfected with the pNolz-IRES2-DsRED plasmid, that was obtained by clonation of the human NolzI contained in the pOTB plasmid (MGC full-length (IRAU) collection, clone ID 4053098) into EcoRI and SmaI restriction sites of p-IRES2-DsRED-Express plasmid (BD Biosciences) coding for DsRED fluorescent protein. As a control, we used pIRES2-DsRED-Express empty plasmid. Tranfection was made with 9 μg of NolzI-RED or RED plasmid.
To reduce NolzI expression, three different siRNAs against NolzI mRNA were used (Silencer Pre-designed siRNAs, IDs 89661, 169777, 89565, Ambion, Applied Biosystems, Foster City, CA, USA). Tranfection was made with 2 μM of each siRNA or 6 μM of negative control siRNA (Silencer Negative Control #1 siRNA, Ambion).
Low passage (four to seven) embryonic neurospheres were disaggregated and transfected by nucleofection following the manufacturer's protocol (Amaxa Biosystems, Lonza Iberica SA, Barcelona, Spain). Using the A33 Nucleofector program (Amaxa Biosystems), 5 × 106 cells were transfected. Viable cells were counted by trypan blue exclusion in a Neubauer chamber after nucleofection.
For BrdU incorporation assays, 65,000 cells/cm2 were seeded after nucleofection. Two days later cells were collected and incubated for 10 minutes in 24-well plates with Matrigel-treated coverslips and they were incubated for 10 minutes in BrdU-containing media at a final concentration of 2 μg/ml. Just after incubation, cells were fixed and processed for immunocytochemistry.
The cell cycle exit index was analyzed as described elsewhere . Briefly, we performed the same procedure as for BrdU incorporation except that neurospheres were pulsed with BrdU the same initial day of inducing hNolz over-expression and cells were fixed 3 days later. Thereafter, neurosphere cultures were processed for BrdU and Ki67 immunostaining. BrdU-positive but Ki67-negative cells were counted as the cells that left the cell cycle during the experimental period.
In order to analyze cell cycle duration, 10 neurospheres were plated 3 days after transfection in 96-well plates with complete medium and supplemented with 1 μM BrdU. Neurospheres were attached at 1, 3, 6, 12 and 24 hours after treatment in 96 well-plates pre-coated with Matrigel. Ten minutes later, cells were fixed in 4% PFA and processed for immunocytochemistry.
For the self-renewal assay, 65,000 cells/cm2 were seeded after nucleofection and the total number of neurospheres obtained 5 days later was counted (passage 0 (P0) after transfection). Cells were dissociated and 2,500 cells/cm2 were seeded and counted again on day 5 (passage 1 (P1) after transfection).
For differentiation after nucleofection, 50,000 cells/cm2 were seeded and the same protocol as for non-nucleofected cells was followed.
To over-express Nolz1 in primary cultures, we transfected the cells with the pLV-Nolz-IRES-EGFP plasmid or the pLV-IRES-EGFP plasmid, which encode hNolz and EGFP or EGFP only, respectively. The pLV-IRES-EGFP plasmid was generated using the pRRLsinPPT plasmid (pRRL) constructed by the Miami Project to Cure Paralysis Viral Vector Core Lab based on the lentiviral transducing plasmid developed by Naldini et al. . Briefly, the multiple cloning site (MCS) of the pRRL plasmid was substituted by the MCS-IRES-EGFP from the PRV-IRES-EGFP (Genetrix SL, Tres Cantos, Madrid, Spain) using the BamHI and the SalI restriction sites. To construct the pLV-Nolz-IRES-EGFP, the hNolz gene from the pNolz-IRES2-DsRED plasmid was cloned into pLV-IRES-EGFP between the MCS BamHI and XhoI sites. Primary cultures were transfected 24 hours after seeding with 0.5 μg of the corresponding plasmids per well (24-well plate). The transfection was performed using Lipofectamine LTX (Invitrogen SA), following the manufacturer's instructions. Three days after transfection cells were fixed with 4% PFA for immunocytochemistry analysis.
For DEAB (Sigma Chemical Co.) treatment, primary cultures were transfected 12 h after seeding as described above. Then, 24 h later DEAB was added to the medium at a concentration of 10-8 M. Three days after treatment cells were fixed with 4% PFA for immunocytochemistry analysis.
For RAR inverse agonist administration, primary cultures were transfected 12 h after seeding as described above. Thereafter, the RAR inverse agonist (BMS493 ) was added to the medium at a concentration of 10-8 M in DMSO, which was repeated every single day. At 3 DIV cells were fixed with 4% PFA for immunocytochemistry analysis.
To over-express Gsx2, the human Gsx2 gene from the pcDNA-hGsx2 plasmid, kindly provided by Dr Peter Marynen (Université de Leuven, Belgium), was PCR-cloned into the retroviral vector pRV-IRES-EGFP using the MCS BamHI and XhoI sites.
For retrovirus production, 293T cells were plated at a density of approximately 6 × 104 cells per cm2. The following day, cells were transfected by a three-plasmid system (the pRV-Gsx2-IRES-GFP plasmid, the plasmid that expresses HIV-1 gag and pol genes, and the plasmid that expresses vesicular stomatitis virus G) using the calcium phosphate/DNA co-precipitate method. The transfection mixture remained on the cells for 7 h before the transfection medium was replaced with fresh medium. The supernatant from vector-producing 293T cells was recovered every 22 h during 3 days before being harvested, passed through a 0.45-μm-pore-size filter to remove producer cells, and then subjected to two centrifugations at 4°C and 22,000 × g for 90 minutes to concentrate the virus. The virus-containing pellet was dissolved in 1% bovine serum albumin. Viral concentrate (20 μl) from pRV-Gsx2-IRES-EGFP or pRV-IRES-EGFP was used to transduce 3.5 × 106 dissociated NPCs in a 6-well plate as described previously . Transduced NPCs were growth as neurospheres as described above for 5 DIV before being pelleted for RNA extraction.
Anti-Nolz1 polyclonal antibodies were obtained from the serum of immunized rabbits with a keyhole limpet hemocyanin (KLH)-conjugated oligopeptide coding for amino acids 2 to 14 of the Nolz1 sequence (MSTAPSLSALRSSKH; Figure Figure1A).1A). Pre-immune serum was obtained from the same rabbits before immunization.
All immunostaining was performed using the following antibodies: polyclonal anti-NolzI (1:10,000), monoclonal anti-GFAP (1:500; Sigma Chemical Co.), monoclonal anti-Tuj1 (1:500; Sigma Chemical Co.), monoclonal anti-BrdU (1:50; Dako A/S, Glostrup, Denmark), monoclonal anti-MAP2 (1:200; Sternberger Monoclonals, Lutherville, MD, USA), polyclonal anti-nestin (Rat 401; 1:40; Developmental Studies Hybridoma Bank; The University of Iowa, Iowa), polyclonal anti-Tle4 (1:200; generous gift from Dr Stefano Stifani, McGill University), polyclonal conjugated FITC-GFP (1:200; ABCAM, Cambridge, UK), polyclonal anti-Ki67 (1:200; Thermo Fisher Scientific SLU, Alcobendas, Madrid, Spain). For Nolz negative controls, pre-immunization serum was used at the same concentration as NolzI antibody-containing serum. Preparations were counterstained with DAPI to visualize the nucleus.
No signal was detected in control immunostaining assays in which the primary antibody was omitted.
We analyzed the expression of several genes by radioactive in situ hybridization as described elsewhere . The following oligonucleotide probes were used: mouse NolzI - complementary to nucleotides 3,226 to 3,266 of the NolzI sequence (GenBank accession number NM_145459); mouse Tle1 - complementary to nucleotides 1,942 to 1,983 of the Tle1 sequence (GenBank accession number NM_011599); mouse Tle2 - complementary to nucleotides 1,351 to 1,389 of the Tle2 sequence (GenBank accession number NM_019725); mouse Tle3 - complementary to nucleotides 3,434 to 3,474 of the Tle3 sequence (GenBank accession number NM_001083927); mouse Tle4 - complementary to nucleotides 1,614 to 1,652 of the Tle4 sequence (GenBank accession number NM_0011600).
Expression of several genes was evaluated by Q-PCR assays performed as previously described , using the following TaqMan® gene expression assays (Applied Biosystems): 18S, Hs99999901_s1; nestin, Mm00450205_m1; β-tubulin III, Mm00727586_s1; GFAP, Mm00546086_m1; MAP2, Mm00485230_m1; Gsx2, Mm00446650_m1; mouse NolzI, Mm00520908_m1; Raldh3, Mm00474049_m1; RARα, Mm00436264_m1; RARβ, Mm01319674_m1; RARγ, Mm00441083_m1; CRBP1, Mm00441119_m1; Cyp26b1, Mm00558507_m1; Tle4, Mm01195160_m1. To specifically recognize hNolz, a customized Taqman® Assay was designed consisting of the following primers: forward, CCTCGCCCTCCTCCAAAC; reverse, GCCCGATTTGGTGTCCTTGT; reporter, TCTCCTCGGTTGCCTCC. To provide negative controls and exclude contamination by genomic DNA, the reverse transcriptase was omitted in the cDNA synthesis step, and the samples were subjected to the PCR reaction with each TaqMan® gene expression assay.
Analysis and quantification was performed with the Comparative Quantitation Analysis program of the MxPro™ Q-PCR analysis software version 3.0 (Stratagene, La Jolla, CA, USA), using the 18S gene expression as internal loading control. All Q-PCR assays were performed in duplicate and repeated for at least three independent experiments. The results were expressed as relative levels with respect to the expression of the same gene in the control condition, considered as 100%.
We analyzed the levels of Nolz1 protein in transfected neurospheres or in the striatum at different developmental stages. Samples (at least n = 3 per time point) were prepared and processed for western blotting as described elsewhere . Blots were incubated overnight at 4°C with anti-NolzI antibody (1:50,000). The secondary antibody was a horse radish peroxidase-conjugated anti-rabbit IgG (1:3,000; Promega Biotech Iberica, SL., Madrid, Spain) and the signal was developed using the ECL western blotting analysis system (GE Healthcare Europe GMBH, Cerdanyola del Vallès, Barcelona, Spain).
In order to determine the role of NolzI on the proliferation of progenitor cells in vitro, we counted the number of cells that incorporate BrdU. BrdU- and EGFP-positive (transfected) cells were detected by immunocytochemistry and the total number of cells determined by DAPI counterstaining. For over-expressing experiments the results were expressed as the percentage of proliferating cells with respect to the transfected (EGFP-positive) cells, while for siRNA experiments, the results were expressed as the percentage of proliferating cells with respect the total number of cells (n = 5). We also counted by phase contrast the total number of neurospheres 5 days after hNolz or control transfection.
Cell death was evaluated by counting the number of apoptotic nuclei stained with DAPI after hNolz over-expression. The results were expressed as the percentage of dying cells with respect to transfected (EGFP-positive) cells (n = 4). Results were normalized with respect to control-transfected NSCs (considered as 100%).
We estimated the cell cycle time as previously described [1,29]. Briefly, BrdU was added to neurosphere cultures during the last 1, 3, 6, 12 and 24 h of culturing. The number of BrdU-positive cells and the total number of cells, determined by DAPI counterstained nuclei, in each neurosphere was counted. The percentage of proliferating cells was calculated for each time point after BrdU administration. Regression analyses of the active portion of each BrdU labeling curve were used to estimate cell cycle time assuming that all cells proliferate at the same rate and that every cell is labeled at the end of a single cycle . The r2 of this lineal correlation was used to calculate the cell cycle duration. We counted at least 30 neurospheres in each condition in 3 transfected cultures.
We analyzed the cell cycle index as the number of cells that retain BrdU but leave the cell cycle (Ki67-negative cells) after a 3-DIV pulse label. Thus, we counted the fraction of BrdU+/Ki67- cells and normalized to the total number of BrdU-positive cells in the culture. Results were expressed as absolute percentages in each condition.
To determine the effect of Nolz1 on the differentiation of LGE primary cultures, we counted the number of cells per coverslip overexpressing hNolz or EGFP that colocalized with different markers, such as nestin, Tuj1 and MAP2 3 or 5 days after the transfection. The results are expressed as the percentage of transfected cells colocalizing with the different markers with respect to the total number of transfected cells. Between 50 and 200 transfected cells per coverslip were counted per transfection (n = 3 to 5).
Coronal brain slices (250 μm) from E14.5 mice embryos were obtained with a vibratome. Slices were plated onto culture membranes with minimum essential medium supplemented with 10% FBS and 50 U/ml penicillin-streptomycin. After 1 hour in the incubator, media was changed to Neurobasal supplemented with B27, 1 mM HEPES, 50 U/ml penicillin-streptomycin and 2 mM L-glutamine. Two hours later, slices were electroporated with 8 μg of DsRED-Nolz or DsRED plasmid. After 48 hours in culture, electroporated slices were fixed during 2 hours with 4% PFA, dehydrated with increasing ethanol concentrations and stored until processing for immunohistochemistry.
We counted the number of Ki67-positive cells present in the electroporated zone of brain slices. First, we took a picture of the slices showing the RED fluorescence of the electroporated plasmids prior to fixation. Then, the slices were immunostained against Ki67 and the number of positive cells included in the electroporated area for the control side (DsRED plasmid) or experimental side (Nolz1-DsRED) were counted. The area to count was fixed by delineating the electroporated DsRED positive area in the pre-immunostaining image using ImageJ, and transferring this area to the Ki67 stained image. At least four different slices were counted for each condition.
To monitor the RARE activity we used the Cignal RARE Reporter Assay Kit (SABioscience Corporation, Frederick, MD, USA) following the manufacturer's instructions. Mixed neuron-glial LGE primary cultures were performed as described above and 24 hours after seeding cells were transfected with the inducible RARE-responsive mixture and the pLV-Nolz-IRES-EGFP or the pLV-IRES-EGFP plasmids. The transfection was performed using Lipofectamine LTX (Invitrogen SA) following the manufacturer's instructions. Two days later, cultures were processed to evaluate luciferase using the Dual-Luciferase Reporter Assay System (Promega). The firefly/Renilla luciferase ratio was calculated for each well, and results are expressed as the mean of four independent experiments and normalized with respect to control-transfected primary cultures (considered as 100%).
All results are expressed as the mean of independent experiments ± standard error of the mean. Results were analyzed using the Student's t-test or one-way ANOVA followed by the Bonferroni post-hoc test.
BrdU: bromodeoxyuridine; DEAB: 4-diethylaminobenzaldehyde; DIV: days in vitro; dLGE: dorsal LGE; DMSO: dimethyl sulfoxide; E: embryonic day; EGFP: enhanced green fluorescent protein; elB: elbow B; FBS: fetal bovine serum; GFAP: glial fibrillary acidic protein; GFP: green fluorescent protein; Gro: Groucho; hNolz: human Nolz; LGE: lateral ganglionic eminence; MAP: microtubule-associated protein; MCS: multiple cloning site; MZ: mantle zone; NET: NocA-Elbow (elB)-Tlp; NPC: neural progenitor cell; PFA: paraformaldehyde; Q-PCR: quantitative PCR; RA: retinoic acid; Raldh: retinaldhehyde dehydrogenase; RAR: RA receptor; RARE: RA response element; siRNA: small interfering RNA; SVZ: subventricular zone; TLE: NocA-elB-Tlp; Tuj1: β-III tubulin; vLGE: ventral LGE; VZ: ventricular zone.
The authors declare that they have no competing interests.
NU, collection and assembly of data, data analysis and interpretation, manuscript writing, final approval of manuscript; RM-I, CH, ME, EC, MP, HRM-G, RW, CC, SA, RA, collection and assembly of data, final approval of manuscript; GD, KC, ARdL, CV-A, SM, JA, financial support, data analysis and interpretation, final approval of manuscript; JMC, conception and design, financial support, administrative support, data analysis and interpretation, manuscript writing, final approval of manuscript.
We would like to thank M Teresa Muñoz, Ana López and Josep Barrachina for technical assistance, and Dr Maria Calvo, Anna Bosch and Neus Abella from the confocal microscopy unit at the Serveis Científico-Tècnics (Universitat de Barcelona) for their support and advice on confocal techniques. We also thank Dr Peter Marynen (Université de Leuven, Belgium) for the pcDNA-hGsx2 construct and Dr Pantelis Tsoulfas (University of Miami, FL, USA) for the pRRLsinPPT plasmid. We thank Dr Stefano Stifani (McGill University, Montreal, Canada) for the anti-Tle4 antibody. We are also grateful to Dr A Nagy, R Nagy, Dr J Rossant, and Dr W Abramow-Newerly from the Samuel Lunenfeld Research Institute (Mont Sinai Hospital, Toronto, Canada) for the generous gift of the R1 mouse embryonic stem cell line. This study was supported by grants from the Ministerio de Ciencia e Innovación (SAF2008-04360, to JA; SAF2009-07774 and PLE2009-0089, to JMC; SAF2004-05798, to CV-A), Spain; Instituto de Salud Carlos III, Ministerio de Ciencia e Innovación (CIBERNED, to JA and CV-A; and RETICS (RD06/0010/0006; Red de Terapia Celular), to JMC), Spain; the Fundació La Marató de TV3 (to JA), Spain; Generalitat de Catalunya (2009SGR-00326 to JA), Spain; and the National Institutes of Health (EY013969, to GD). The Cell Therapy Program is supported by the Centre of Regenerative Medicine in Barcelona (CMRB; Promt-0901, to JMC; Generalitat de Catalunya), Spain.