- Research article
- Open Access
The neuroblast and angioblast chemotaxic factor SDF-1 (CXCL12) expression is briefly up regulated by reactive astrocytes in brain following neonatal hypoxic-ischemic injury
- Jason T Miller1,
- John H Bartley2, 3,
- Hereward JC Wimborne1, 3,
- Aisha L Walker3, 4,
- David C Hess1, 3,
- William D Hill†1, 3, 4Email author and
- James E Carroll†1, 3Email author
© Miller et al; licensee BioMed Central Ltd. 2005
Received: 10 May 2005
Accepted: 31 October 2005
Published: 31 October 2005
Stromal cell-derived factor 1 (SDF-1 or CXCL12) is chemotaxic for CXCR4 expressing bone marrow-derived cells. It functions in brain embryonic development and in response to ischemic injury in helping guide neuroblast migration and vasculogenesis. In experimental adult stroke models SDF-1 is expressed perivascularly in the injured region up to 30 days after the injury, suggesting it could be a therapeutic target for tissue repair strategies. We hypothesized that SDF-1 would be expressed in similar temporal and spatial patterns following hypoxic-ischemic (HI) injury in neonatal brain.
Twenty-five 7-day-old C57BL/J mice underwent HI injury. SDF-1 expression was up regulated up to 7 days after the injury but not at the later time points. The chief sites of SDF-1 up regulation were astrocytes, their foot processes along blood vessels and endothelial cells.
The localization of SDF-1 along blood vessels in the HI injury zone suggests that these perivascular areas are where chemotaxic signaling for cellular recruitment originates and that reactive astrocytes are major mediators of this process. The associated endothelium is likely to be the site for vascular attachment and diapedesis of CXCR4 receptor expressing cells to enter the injured tissue. Here we show that, relative to adults, neonates have a significantly smaller window of opportunity for SDF-1 based vascular chemotaxic recruitment of bone marrow-derived cells. Therefore, without modification, following neonatal HI injury there is only a narrow period of time for endogenous SDF-1 mediated chemotaxis and recruitment of reparative cells, including exogenously administered stem/progenitor cells.
Hypoxic-ischemic (HI) injury to the brain is a significant cause of neurological morbidity in infants. The resultant severe and longstanding disability to infants has provided impetus for exploring aggressive therapies that give promise of injury reversal. Transplantation of stem cells has emerged as a possible modality to help improve function in damaged tissues .
In organ-specific injury models, bone marrow cells have been shown to accumulate at the site of injury and to differentiate into tissue specific cells [2–5]. Chen and colleagues  reported that intravenously administered marrow stromal cells accumulate in the site of ischemic brain injury, with a small percentage expressing neuronal markers. Additionally, Hess et al. [7, 8] have demonstrated that, following temporary ischemia, endogenous murine bone marrow cells give rise to perivascular/mural cells, microglial cells, and a limited number of cells positive for the neuronal marker, NeuN. However, it is unclear if the NeuN positive cells develop into mature neurons.
Among the milieu of chemicals expressed in the injured microenvironment, the chemotactic chemokine, stromal cell derived factor-1 (SDF-1 or CXCL12), has emerged as a major attractant of reparative cells. SDF-1 and its receptor, CXCR4, play a critical role in both engraftment of hematopoietic stem cells into bone marrow and the mobilization of stem/progenitor cells from bone marrow niches into the peripheral circulation where these cells are then available for delivery to sites of peripheral injury [9–11]. In addition to functioning in the hematopoietic system, CXCR4 positive cells respond to SDF-1 signals in non-hematopoietic injured organs . That exogenous bone marrow-derived cells home to and migrate within the site of injury suggests that the brain's response to injury produces signals that attract these cells [7, 8, 13]. Functionally, SDF-1 is a powerful chemoattractant for CXCR4-expressing bone marrow derived cells, including putative bone marrow stem/progenitor cells such as CD34+ cells both in vitro and in vivo .
In addition to targeting hematopoietic cells, the SDF-1/CXCR4 system is also known to play a critical role in embryonic brain development and adult injury repair including neurogenesis, neuroblast migration, and neuronal organization as well as endothelial progenitor cell recruitment, endothelial cell migration and vasculogenesis [15–25].
Therefore, it is important to determine the spatial and temporal expression of SDF-1 relative to injury; SDF-1 expression patterns may establish not only the location and duration of the window of opportunity for endogenous injury-mediated chemotaxis of reparative cells, but also the timeframe for therapeutic transplantation and recruitment of various stem cell populations. Recently, we showed in an adult mouse model of stroke that SDF-1 is expressed perivascularly in the injured region up to 30 days after middle cerebral artery occlusion , suggesting that there may be a long post-injury window for homing of reparative cells. Anticipating that SDF-1 might be a critical factor in attracting transplanted cells to the injured area of the neonatal brain, we hypothesized that SDF-1 would be expressed in neonatal hypoxic-ischemic injury in a temporal and spatial pattern similar to that seen in adult models of ischemic brain injury.
Spatial expression pattern of SDF-1 in uninjured brain
Changes in spatial expression following HI injury
Temporal expression pattern of SDF-1 following HI injury
The first day after HI injury (P8) patchy SDF-1 expression was demonstrated around blood vessels and within the parenchyma in the hippocampus and striatum within the ischemic hemisphere. By 3 days after HI injury (P10) there was robust, uniform hippocampal expression of SDF-1 in the CA1, CA2, CA3 and dentate regions as well as within the striatum and to a limited degree in the cingulate cortex (Figures 5, 6, 7). By day 5 after the injury (P12) SDF-1 continued to be expressed but was significantly reduced in the hippocampus and striatum. However, its expression was still increased in the choroid plexus (bilaterally) and was associated with blood vessels in the white matter of the corpus callosum and external capsule as well as pial mesothelial cells (bilaterally). By day 7 (P14), SDF-1 expression continued to wane, and by day 10 post-HI injury (P17) and beyond, expression was reduced below observable levels in the hippocampus, striatum and cortical areas. The only expression of SDF-1 at these late times was found along white matter tracts of the corpus callosum and the alveus and in some sites where normal constitutive expression is observed, specifically the subventricular zone, choroid plexus and a subset of large cingulate cortex and neocortical neurons. However, expression appeared to be depressed in hippocampal areas that normally expressed SDF-1.
Cellular expression of SDF-1
The regulation of SDF-1 may be critical to the incorporation of a variety of new cells into brain. In contrast to the prolonged up regulation of SDF-1 following stroke in adult mice , its up regulation in neonatal mice after HI injury was brief. This may reflect a difference between a mature, relatively stable, adult brain structure and a more plastic, still developing, neonatal CNS where there may be a more active regulation of SDF-1 expression. The timing of post-HI injury SDF-1 expression suggests that SDF-1 mediated cell homing may be most effective from 3 to 5 days after HI injury in neonatal animals, peaking around 3 days. During this time SDF-1 expression is high around vascular elements, which may provide a portal of access for circulating reparative cells to the areas of ischemic injury.
Another possible explanation for the temporal differences of SDF-1 expression between injured adult and neonatal brains may be related to the type of injury. HI injury produces a more diffuse and graded tissue injury, while middle cerebral artery occlusion is more focal and discrete.
Constitutive SDF-1 expression
Interestingly, the pattern of peak expression for SDF-1 we show at postnatal day 10, 3 days after HI injury (Figure 6), is virtually identical to that recently published by Felszeghy et al for I125 SDF-1α binding to CXCR4 in a rat HI model, 2 days after HI injury, at postnatal day 9 . In Felszeghy et al's study the localization of CXCR4 receptors suggests the distribution of SDF-1 expression. Protein expression observed in our study, with SDF-1 antibody probes, is consistent with mRNA expression patterns assayed by in situ hybridization in previous reports with some exceptions [26–28]. The SDF-1 mRNA expression patterns Tham et al and Stumm et al [22, 23] show at days P7 and P9 in rats match protein expression patterns we detected here at P8 and P10 in mice (Figures 3, 5 and 6). This includes SDF-1 expression in the meninges, the hippocampal fissure, choroid plexus and the proliferative subventricular zone. SDF-1 mRNA expression in both in situ hybridization studies [22, 23] was also associated, to a limited degree, with blood vessels, we saw the same constitutive pattern for SDF-1 immunostaining particularly with vessels associated with the hippocampal fissure and with white matter tracks (Figure 3). In the in situ hybridization studies [22, 23] there is a decline in hippocampal fissure SDF-1 mRNA expression between the early time points (P7 & P9) and later time points (P14 and P12 – P21). A similar decrease in hippocampal fissure SDF-1 immunostaining was observed in our study between P8 and P14 (Figures 3 and 4). Of interest, in the in situ hybridization studies [22, 23], there are consistent increases in SDF-1 mRNA in the dentate gyrus granular layers, in CA3 (and CA4) and in layer V neocortical neurons between the early time points (P7 & 9) and later time points (P14 and P12 – P21). However, we did not detect significant SDF-1 immunolabelling over the cell bodies of the granular cells at equivalent time points in the mice (P8 – 14). In contrast we did detect immunolabelling in the molecular and polymorph layers, regions of granular cell dendritic arborizations and axon fields . This labelling increased between P8 and P14 (Figures 3 and 4). Similarly we did not detect strong SDF-1 immunoreactivity over CA 3, 2 or 1 neuronal somas, but we found immunoreactivity that increased between P8 and P14 in the hippocampal lacunosum molecular layer, the stratum radiatum and the oriens layer (Figures 3 and 4), regions that contain the dendritic and axonal fields for the CA region . Additionally, the layer V neocortical neurons are reported to show strong mRNA labelling [22, 23], but we only detected weak diffuse antibody labelling in the area corresponding to layers V and VI in the neocortex (Figure 3).
The discrepancy between the reported neuronal somal labelling for mRNA [22–24] and the neuropil immunolabelling for SDF-1 protein we observed may be due to a lack of sensitivity of the antibody, although we can clearly detect SDF-1 expressing structures that are reported to express lower levels of SDF-1 mRNA than dentate gyrus granular cells, CA and layer V neocortical neurons [22, 23]. There may also be differences in SDF-1 transcription and translation rates as well as message and protein turnover in different cell populations. Alternatively, this may reflect that SDF-1 mRNA is synthesized in, and restricted to, the neuronal somas while in some neurons the protein product is mainly exported to cellular processes with little remaining in the somas. For example, while the reported dentate gyrus granular cell mRNA expression [22–24] is more intense than any other location, including the hippocampal fissure, we show that this is at best poorly labelled immunohistochemically (Figures 3 and 4). In contrast we demonstrate that regions that reflect the synaptic fields (dendritic and axonal) of the granular cells (molecular and polymorph layers) have strong immunoreactive expression for SDF-1 (Figures 3 and 4) while these same regions show little mRNA expression for SDF-1 [22–24]. Further, structures lacking projecting processes, which could distance mRNA form protein localization, like the hippocampal fissure, choroid plexus, and meninges, are reported to be strongly labelled for SDF-1 mRNA by in situ hybridization [22–24] and we demonstrate also by immunohistochemistry for the SDF-1 protein. There is precedent for this type of pattern in neonatal hippocampus. Czarnecki et al have recently shown that synaptopodin mRNA was restricted to dentate granular layer, and CA3, cell somas while immunostaining for synaptopodin protein labeled dendritic layers but not the somas .
Injury induced SDF-1 expression
Recently Ceradini et al. demonstrated that SDF-1 gene expression is regulated by the hypoxia responsive transcription factor HIF-1 . The level of SDF-1 expression is directly related to the degree of hypoxia such that hypoxic gradients within tissues correlate with gradients of SDF-1 gene expression . We have previously shown in an adult middle cerebral artery occlusion model of stroke that SDF-1 expression follows a gradient pattern consistent with the hypoxia gradient in the penumbra . In our neonatal HI model the hippocampus did not appear to show a gradient of SDF-1 labeling during peak expression, rather the labeling was uniform and delimited by anatomical boundaries. In contrast the striatal expression did appear to show a gradient of labeling intensity (Figure 6). Specific cell types may be more sensitive to hypoxic changes in inducing SDF-1 expression as illustrated by changes in constitutive expression of SDF-1 as well as induced expression in cells that did not show significant constitutive expression. For example, subsets of neocortical neurons responded by decreasing SDF-1 expression in both the hypoxic and HI affected hemispheres while choroid plexus and pial labeling increased on both sides and astrocytes dramatically expressed SDF-1 only in the HI hemisphere. This suggests that HIF-1 expression may be differentially induced or that other transcription factors may be involved as well.
Potential role of SDF-1 in injury repair
SDF-1 and its receptor CXCR4 are emerging as a common axis for directing the migration of stem cells associated with injury repair in many systems. Ji et al recently demonstrated that SDF-1 mediates the migration of mesenchymal stem cells to the site of injury . Neural progenitor cells and neuroblasts express CXCR4 and are attracted by SDF-1α developmentally and following brain ischemia [25, 30–32]. Recently SDF-1 has been shown to promote neovascularization in somatic tissues and to recruit bone marrow-derived (BMD) cells to areas of ischemic injury. In mouse models of peripheral tissue ischemia, SDF-1 treated animals had increased capillary density and blood flow compared to controls and recruited injected endothelial precursor cells (EPC) to integrate into blood vessels demonstrating vasculogenesis [16, 20, 21]. Importantly this SDF-1 induced neovascularization has been demonstrated to improve perfusion and function in peripheral tissue ischemic injury models [16, 21, 33]. Work from our laboratory shows SDF-1 is up regulated in the penumbral, or peri-infarct, zone within hours of acute ischemia in adult mice. This elevated expression persists in the peri-infarct zone for at least 30 days post-ischemia. Accompanying this we observe bone marrow-derived cell infiltration, pericyte and microglial engraftment and neovascularization . Given the apparent function of SDF-1 to serve as an attractant for bone marrow-derived cells, including cells associated with vascular repair and vasculogenesis, as well as for other stem/progenitor cells, including neural stem cells, this brief time span of SDF-1 expression, peaking at 3 days with only limited expression through 7 days after the injury in neonatal animals, may be critical for the acquisition of new brain or reparative cells.
The cell type expressing SDF-1 and its localization is highly related to its function. Previously, we found that the principal localization of SDF-1 expression following injury was astrocytic, often strongly associated with small blood vessels . This was the first demonstration that activated, or reactive astrocytes, express SDF-1 in vivo following ischemia injury . The current study confirms and extends our original finding and demonstrates that SDF-1 expression is massively up regulated in reactive astrocytes in neonatal HI injury, but for a shorter period of time relative to adult middle cerebral artery occlusion ischemia. Recently Imitola  also reported SDF-1 expression in reactive astrocytes in an adult HI model. Earlier in vitro studies showed that cultured astrocytes up regulate SDF-1 expression following exposure to various cytotoxic or inflammation-inducing agents [34, 35]. Additionally, we have recently shown that there is only minimal proliferation and maturation of astrocytes following HI, suggesting that the astrocytic expression of SDF-1 following HI originates from existing astrocytes .
The influence of SDF-1 upon ischemic recovery in neonates appears to be restricted to a few days under circumstances of "normal" endogenous repair. Such a brief up regulation of SDF-1 in neonatal animals may disadvantage their recovery relative to adults. However, it may still may provide a defined time frame in which therapeutically transplanted cells, or autologous stem cells mobilized from the bone marrow, may be able to home, engraft and differentiate into needed cell types. This may also provide an opportunity to target engineered cells that express specific factors to the site of injury. Using the SDF-1/CXCR4 axis as a vectoral targeting system may also permit local application of cell expressed therapeutic factors in higher doses than systemic delivery would safely allow. In adults it may be possible to use the natural up regulation of the SDF-1 for up to 30 days after the injury, while in neonates such a procedure would have to be carried out much sooner. If transplantation protocols are carried out in humans, it may be necessary to find ways of either up regulating the SDF-1 or engineering the expression of the chemokine to desired temporal and spatial locals.
SDF-1 up regulation following neonatal HI injury persists only a few days in comparison to the much longer up regulation in adult models of stroke. The up regulation in neonatal HI injury is quite prominent in astrocytes abutting small blood vessels. This process may be critical in attracting CXCR4 expressing cells to the brain. Awareness of these events could be helpful in planning stem cell transplantation therapy delivered via the vascular route.
This study was performed in accordance with the guidelines provided by the Laboratory Animal Studies Committee of the Veterans Administration Medical Center (Augusta, GA) and the Medical College of Georgia. The mice were housed in individual cages under standard conditions. Offspring were reared with their dams until the time of surgery, and then until weaning at three weeks of life.
Surgical procedure and treatment
Twenty-five C57 BL/6 mouse pups underwent permanent ligation of the left common carotid artery at post-natal day seven (P7) . A midline cervical incision was made to expose the left common carotid artery, and a single suture ligated the artery. The incision was closed with interrupted 6-0 silk sutures. During the procedure, the mice were anesthetized with 2% isoflurane. The pups were then placed with the dams for two hours prior to placement in an 8% oxygen chamber partially immersed in a water bath at 37° for 75 minutes.
Animal sacrifice and tissue processing
The pups were sacrificed at P8, P10, P12, P14, P17, P21, or P35 (respectively, 1, 3, 5, 7, 10, 14 or 28 days after the injury). At least three animals were sacrificed at each time point. At the time of sacrifice, the animals were anesthetized with 70 mg/kg of ketamine and 15 mg/kg xylazine. Tissue was fixed by transcardiac perfusion with 0.9% saline, followed by 4% paraformaldehyde in PBS. Brains were removed and post-fixed in 4% paraformaldehyde for 4 hours, cut into 3–5 mm sections, and continued in 4% paraformaldehyde for an additional 20 hours. Tissue was then dehydrated in an ethanol series, cleared in xylene, and infiltrated and embedded in PolyFin Embedding and Infiltration Wax (TBS Biomedical Sciences, Durham, NC). Paraffin embedded tissue was sectioned 5 μ thick and mounted on Superfrost Plus slides (Fisher Scientific).
Section processing, antigen retrieval and immunostaining methods have been previously described [13, 36] Briefly, slide mounted sections were deparaffinized through 3 xylene changes followed by rehydration in an alcohol dilution series. Sections were permeablized in 0.1% Triton-X 100 in PBS for ten minutes, followed by 3 washes in 1× PBS. Antigen retrieval was performed using a microwave defixation method. Slides were microwaved at a slow boil for 10 minutes in citrate buffer (0.01 M sodium citrate pH 6.5) then incubated at rest for twenty minutes, then washed in 3 changes of 1× PBS and blocked using 2% normal calf serum in PBS for 20 minutes at room temperature (RT).
Sections were labeled with antibodies to SDF-1 (Santa Cruz cat # sc-6193, goat, recognizes both SDF-1α & β splice variants). SDF-1 signal was detected by utilizing either a biotin/avidin (Vector Elite ABC kit) or peroxidase anti-peroxidase (PAP; Sternberger) amplification system and visualized with Cy3 conjugated antibody (Jackson ImmunoResearch Laboratories). In some instances dual labeling for SDF-1 and a second antigen was utilized to identify the phenotype of SDF-1 expressing cells. For co-labeling SDF-1 and the astrocyte marker glial fibrillary acidic protein (GFAP) a rabbit anti-GFAP antibody (DAKO cat# Z0334) was used, for oligodendricytes anti-CNPase (Sigma cat# C5922, mouse) and the biotinylated lectin Ricinus Communis Agglutinin I (RCA 1, Vector cat# B-1085, detects unblocked N-Acetyl galactosamine and galatose) for the visualization of endothelial cells and microglial cells [13, 36]. All antibodies (and RCA-1) were allowed to incubate at room temperature for one hour and washed four times (1× PBS 5 minutes each). All primary antibodies were detected using indirect staining with a secondary, fluorescent antibody. Cy3 anti-Goat (Jackson # 705-165-147), diluted 1:400, was used to visualize SDF-1 in all cases. FITC anti-rabbit (Jackson # 711-095-152), diluted 1:100, was used to visualize GFAP. Strepavidin FITC (Jackson #016-010-084), diluted 1:100, was used to visualize biotinylated RCA. FITC anti-mouse (Jackson #715-095-151), diluted 1:100, was used to visualize CNPase. Slides were rinsed in 4 changes of PBS for 5 minutes each. Negative controls consisted of preabsorbing 660 ng/ml, (4.3 pM/ml) the SDF-1 antibody (Santa Cruz cat # sc-6193, goat) with 1.5 ng/ml (43 pM/ml) of recombinant murine SDF-1α (Peprotech # 250-20A) at 37°C for 1 hour prior to use or leaving off the primary antibody. Cell nuclei were counterstained with bis-benzimide (Sigma, 10 mg/ml stock diluted 1:12,000 in phosphate buffered saline) for 8 minutes then given a final wash prior to coverslipping with Vectashield mounting media (Vector Labs #H-1000).
Recombinant murine SDF-1α (25 & 100 ng) was run on a Novex NuPage 10% Bis-Tris Gel (Invitrogen NP0302BOX) with MES buffer at 75 volts then transferred to a 0.2 um PVDF membrane (Millipore Immobilon PSQ #ISEQ00010). The blot was blocked with 4% cold water fish gelatin (Sigma #G-7765) in PBS at room temperature for 1 hour. The SDF-1 antibody (Santa Cruz cat # sc-6193, goat) was incubated shaking (1:100, 10 ug/ml) overnight at 4°C. The blot was rinsed, then washed 2 times for 10 minutes each in PBS with 0.5% Tween-20 (Fisher #BP337-500). The anti-SDF-1 antibody was detected with an anti-goat secondary antibody conjugated with HRP (Jackson ImmunoResearch #705-035-003, 1:50,000) for 1 hour at room temperature. The blot was washed again (3 times for 10 minutes each in PBS with 0.5% Tween-20 and 1 time with PBS only), developed with ECL detection reagent (Amersham # RPN2109D1) and exposed to X-Ray film (Fujifilm Super RX #100NIF).
Confocal imaging was used to confirm dual labeling with a Zeiss 510 laser scanning confocal microscope (Zeiss LTM software) as previously described [13, 36]. The objective used was Zeiss 63× C-Apochromat 1.2NA. To excite the FITC fluorochrome (green), a 488-nm laser line generated by an argon laser was used, and for the Cy3 fluorochrome (red), a 543-nm laser from a HeNe laser was used. Filter sets used were a bandpass 500- to 600-filter ("green" channel) and a long-pass 585- to 650-nm filter ("red" channel). We identified cells that were labeled for SDF-1 and either GFAP or RCA with 1-μm step Z series.
- Bartley J, Carroll JE: Stem cell therapy for cerebral palsy. Expert Opin Biol Ther. 2003, 3: 541-549.PubMedGoogle Scholar
- Ferrari G, Cusella-DeAngelis G, Coletta M, Paolucci E, Stornaiuolo A, Cossu G, Mavilio F: Muscle regeneration by bone marrow-derived myogenic progenitors. Science. 1998, 279: 1528-1530. 10.1126/science.279.5356.1528.View ArticlePubMedGoogle Scholar
- Gussoni E, Soneoka Y, Strickland CD, Buzney EA, Khan MK, Flint AF, Kunkel LM, Mulligan RC: Dystrophin expression in the mdx mouse restored by stem cell transplantation. Nature. 1999, 401: 390-394. 10.1038/43922.PubMedGoogle Scholar
- Petersen BE, Bowen WC, Patrene KD, Mars WM, Sullivan AK, Murase N, Boggs SS, Greenberger JS, Goff JP: Bone marrow as a potential source of hepatic oval cells. Science. 1999, 284: 1168-1170. 10.1126/science.284.5417.1168.View ArticlePubMedGoogle Scholar
- Priller J, Persons DA, Klett FF, Kempermann G, Kreutzberg GW, Dirnagl U: Neurogenesis of cerebellar purkinje neurons from gene-marked bone marrow cells in vivo. J Cell Biol. 2001, 155: 733-738. 10.1083/jcb.200105103.PubMed CentralView ArticlePubMedGoogle Scholar
- Chen J, Li Y, Wang L, Lu M, Zhang X, Chopp M: Therapeutic benefit of intracerebral transplantation of bone marrow stromal cells after cerebral ischemia in rats. J Neurol Sci. 1997, 189: 49-57. 10.1016/S0022-510X(01)00557-3.View ArticleGoogle Scholar
- Hess DC, Hill WD, Martin-Studdard A, Carroll J, Brailer J, Carothers J: Bone marrow as a source of endothelial cells and NeuN-expressing cells after stroke. Stroke. 2002, 33: 1362-1368. 10.1161/01.STR.0000014925.09415.C3.View ArticlePubMedGoogle Scholar
- Hess DC, Abe T, Hill WD, Studdard AM, Carothers J, Masuya M, Fleming PA, Drake CJ, Ogawa M: Hematopoietic origin of microglial and perivascular cells in brain. Exp Neurol. 2004, 186: 134-44. 10.1016/j.expneurol.2003.11.005.View ArticlePubMedGoogle Scholar
- Peled A, Grabovsky V, Habler L, Sandbank J, Arenzana-Seisdedos F, Petit I, Ben-Hur H, Lapidot T, Alon R: The chemokine SDF-1 stimulates integrin-mediated arrest of cd34(+) cells on vascular endothelium under shear flow. J Clin Invest. 1999, 104: 1199-1211.PubMed CentralView ArticlePubMedGoogle Scholar
- Hattorri K, Heissig B, Rafii S: The regulation of hematopoietic stem cell and progenitor mobilization by chemokine SDF-1. Leukemia & Lymphoma. 2003, 44: 575-82. 10.1080/1042819021000037985.View ArticleGoogle Scholar
- Liles WC, Broxmeyer HE, Rodger E, Wood B, Hubel K, Cooper S, Hangoc G, Bridger GJ, Henson GW, Calandra G, Dale DC: Mobilization of hematopoietic progenitor cells in healthy volunteers by AMD a CXCR4 antagonist. Blood. 3100, 102: 2728-30. 10.1182/blood-2003-02-0663.View ArticleGoogle Scholar
- Kollet O, Shivtiel S, Chen Y-Q, Suriawinata J, Thung SN, Dabeva MD, Kahn J, Speigel A, Dar A, Samir S, Goichberg P, Kalinkovich A, Arenzana-Seisdedos F, Nagler A, Izhar I, Revel M, Shafritz DA, Lapidot TH: HGH, SDF-1, and MMP-9 are involved in stress-induced human CD34+ stem cell recruitment to the liver. J Clin Invest. 2003, 112: 160-169. 10.1172/JCI200317902.PubMed CentralView ArticlePubMedGoogle Scholar
- Hill WD, Hess DC, Martin-Studdard A, Carothers JJ, Zheng J, Hale D, Maeda M, Fagan SC, Carroll JE, Conway SJ: SDF-1 (CXCL 12) is up regulated in the ischemic penumbra following stroke: association with bone marrow cell homing to injury. J Neuropath Exp Neurology. 2004, 63: 84-96.Google Scholar
- Auiti AT, Webb IJ, Bleul C, Springer T, Gutierrez JC: The chemokine SDF-1 is achemoattracttant for human CD34+ hematopoietic progenitor cells and provides a new mechanism to explain the mobilization of CD34+ progenitors for peripheral blood. J Exp Med. 1997, 185: 111-120. 10.1084/jem.185.1.111.View ArticleGoogle Scholar
- Lazarini F, Tham TN, Casanova P, Arenzana-Seisdedos F, Dubois-Dalcq M: Role of the α-chemokine stromal cell-derived factor (SDF-1) in the developing and mature central nervous system. GLIA. 2003, 42: 139-148. 10.1002/glia.10139.View ArticlePubMedGoogle Scholar
- Yamaguchi J-I, Kusano KF, Masuo O, Kawamoto A, Silver M, Murasawa S, Bosch-Marce M, Masuda H, Losordo DW, Isner JM, Asahara T: Stromal cell-derived factor-1 effects on ex-vivo expanded endothelial progenitor cell recruitment for ischemic neovascularization. Circulation. 2003, 107: 1322-1328. 10.1161/01.CIR.0000055313.77510.22.View ArticlePubMedGoogle Scholar
- Salcedo R, Wasserman K, Young HA, et al: Vascular endothelial growth factor and basic fibroblast growth factor induce expression of CXCR4 on human endothelial cells: In vivo neovascularization induced by stromal-derived factor-1alpha. Am J Pathol. 1999, 154: 1125-35.PubMed CentralView ArticlePubMedGoogle Scholar
- Mirshahi F, Pourtau J, Li H, et al: SDF-1 activity on microvascular endothelial cells: Consequences on angiogenesis in vitro and in vivo models. Thromb Res. 2000, 99: 587-94. 10.1016/S0049-3848(00)00292-9.View ArticlePubMedGoogle Scholar
- Salvucci O, Yao L, Villalba S, Sajewicz A, Pittaluga S, Tosato G: Regulation of endothelial cell branching morphogenesis by endogenous chemokine stromal-derived factor-1. Blood. 2002, 99: 2703-11. 10.1182/blood.V99.8.2703.View ArticlePubMedGoogle Scholar
- Askari AT, Unzek S, Popovic ZB, Goldman CK, Forudi F, Kiedrowski M, Rovner A, Ellis SG, Thomas JD, DiCorleto PE, Topol EJ, Penn MS: Effect of stromal-cell-derived factor 1 on stem-cell homing and tissue regeneration in ischaemic cardiomyopathy. Lancet. 2003, 362: 697-703. 10.1016/S0140-6736(03)14232-8.View ArticlePubMedGoogle Scholar
- Ceradini DJ, Kulkarni AR, Callaghan MJ, Tepper OM, Bastidas N, Kleinman ME, Capla JM, Galiano RD, Levine JP, Gurtner GC: Progenitor cell trafficking is regulated by hypoxic gradients through HIF-1 induction of SDF-1. Nat Med. 2004, 10: 858-64. 10.1038/nm1075.View ArticlePubMedGoogle Scholar
- Tham TN, Lazarini F, Franceschini IA, Lachapelle F, Amara A, Dubois-Dalcq M: Developmental pattern of expression of the alpha chemokine stromal cell-derived factor 1 in the rat central nervous system. Eur J Neurosci. 2001, 13: 845-56. 10.1046/j.0953-816x.2000.01451.x.View ArticlePubMedGoogle Scholar
- Stumm RK, Zhou C, Ara T, Lazarini F, Dubois-Dalcq M, Nagasawa T, Hollt V, Schulz S: CXCR4 Regulates Interneuron Migration in the Developing Neocortex. J Neurosci. 2005, 23: 5123-5130.Google Scholar
- Lu M, Grove EA, Miller RJ: Abnormal development of the hippocampal dentate gyrus in mice lacking the CXCR4 chemokine receptor. Proc Natl Acad Sci U S A. 2002, 99: 7090-95. 10.1073/pnas.092013799.PubMed CentralView ArticlePubMedGoogle Scholar
- Imitola J, Raddassi K, Park KI, Mueller F-J, Nieto M, Teng YD, Frenkel D, Li J, Sidman RL, Walsh CA, Snyder EY, Khoury SJ: Directed migration of neural stem cells to sites of CNS injury by the stromal cell-derived factor 1a/CXC chemokine receptor 4 pathway. PNAS. 2004, 101: 18117-18122. 10.1073/pnas.0408258102.PubMed CentralView ArticlePubMedGoogle Scholar
- Felszeghy K, Banisadr G, Rostene W, Nyakas C, Haour F: Dexamethasone downregulates chemokine receptor CXCR4 and exerts neuroprotection against hypoxia/ischemia-induced brain injury in neonatal rats. Neuroimmunomodulation. 2004, 11: 404-13. 10.1159/000080151.View ArticlePubMedGoogle Scholar
- Traub RD: Neuronal Networks of the Hippocampus. 1991, Cambridge, Cambridge: University PressView ArticleGoogle Scholar
- Czarnecki K, Haas CA, Orth CB, Deller T, Frotscher M: Postnatal Development of Synaptopodin Expression in the Rodent Hippocampus. J Comp Neurol. 2005, 490: 133-144. 10.1002/cne.20651.View ArticlePubMedGoogle Scholar
- Ji JF, He BP, Dheen TS, Tay SST: Interactions of chemokine receptors mediate the migration of mesenchymal stem cells to the impaired site in the brain after hypoglossal nerve injury. Stem Cells. 2004, 22: 415-427. 10.1634/stemcells.22-3-415.View ArticlePubMedGoogle Scholar
- Ni HT, Hu S, Sheng WS, Olson JM, Cheeran MC-J, Chan ASH, Lokensgard JR, Peterson PK: High-level expression of functional chemokine receptor CXCR4 on human neural precursor cells. Dev Brain Res. 2004, 152: 159-169. 10.1016/j.devbrainres.2004.06.015.View ArticleGoogle Scholar
- Peng H, Huang Y, Rose J, Erichsen D, Herek S, Fujii N, Tamamura H, Zheng J: Stromal cell-derived factor 1-mediated CXCR4 signaling in rat and human cortical neural progenitor cells. J Neurosci Research. 2004, 76: 35-50. 10.1002/jnr.20045.View ArticleGoogle Scholar
- Tran PB, Ren D, Veldhouse TJ, Miller RJ: Chemokine receptors are expressed widely by embryonic and adult neural progenitor cells. J Neurosci Res. 2004, 76: 20-34. 10.1002/jnr.20001.View ArticlePubMedGoogle Scholar
- Hiasa K, Ishibashi M, Ohtani K, Inoue S, Zhao Q, Kitamoto S, Sata M, Ichiki T, Takeshita A, Egashira K: Gene transfer of stromal cell-derived factor-1alpha enhances ischemic vasculogenesis and angiogenesis via vascular endothelial growth factor/endothelial nitric oxide synthase-related pathway: next-generation chemokine therapy for therapeutic neovascularization. Circulation. 2004, 109: 2454-61. 10.1161/01.CIR.0000128213.96779.61.View ArticlePubMedGoogle Scholar
- Bajetto A, Bonavia R, Barbero S, et al: Glial and neuronal cells express functional chemokine receptor CXCR4 and its natural ligand stromal cell-derived factor 1. J Neurochem. 1999, 73: 2348-57. 10.1046/j.1471-4159.1999.0732348.x.View ArticlePubMedGoogle Scholar
- Guillemin GJ, Croitoru-Lamoury J, Dormont D, Armati PJ, Brew BJ: Quinolinic acid upregulates chemokine production and chemokine receptor expression in astrocytes. Glia. 2003, 41: 371-81. 10.1002/glia.10175.View ArticlePubMedGoogle Scholar
- Bartley JH, Soltau T, Wimborne H, Kim S, Martin-Studdard A, Hess DC, Hill WD, Waller JL, Carroll JE: BrdU-Positive Cells in the Neonatal Mouse Hippocampus Following Hypoxic-Ischemic Brain Injury. BMC Neurology. 2005, 6: 15.Google Scholar
- Rice JE, Vannucci RC, Brierly JB: The influence of immaturity on hypoxic-ischemic brain damage in the rat. Ann Neurol. 1981, 9: 131-141. 10.1002/ana.410090206.View ArticlePubMedGoogle Scholar
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