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Nature. Author manuscript; available in PMC Nov 16, 2013.
Published in final edited form as:
PMCID: PMC3667629
NIHMSID: NIHMS455855
Post-injury protective astrogenesis from SVZ niche is controlled by Notch modulator Thbs4
Eric J. Benner,1 Dominic Luciano,2,3 Rebecca Jo,1,2 Khadar Abdi,2 Patricia Paez-Gonzalez,2 Huaxin Sheng,4 David Warner,4 Chunlei Liu,5 Cagla Eroglu,2,6 and Chay T. Kuo1,2,3,6,7
1George and Jean Brumley Neonatal-Perinatal Research Institute, Department of Pediatrics, Duke University School of Medicine, Durham, NC 27710, USA
2Department of Cell Biology, Duke University School of Medicine, Durham, NC 27710, USA
3Department of Neurobiology, Duke University School of Medicine, Durham, NC 27710, USA
4Department of Anesthesiology, Duke University School of Medicine, Durham, NC 27710, USA
5Department of Radiology, Duke University School of Medicine, Durham, NC 27710, USA
6Duke Institute for Brain Sciences, Duke University School of Medicine, Durham, NC 27710, USA
7Preston Robert Tisch Brain Tumor Center, Duke University School of Medicine, Durham, NC 27710, USA
Correspondence: Chay T. Kuo, Departments of Cell Biology, Neurobiology, Pediatrics, Duke University School of Medicine, 366 Nanaline Duke Bldg. Box 3709, 307 Research Drive, Durham, NC 27710, chay.kuo/at/duke.edu
Postnatal/adult neural stem cells (NSCs) within the rodent subventricular/subependymal zone (SVZ/SEZ) generate Doublecortin (DCX)+ neuroblasts that migrate and integrate into olfactory bulb circuitry1,2. Continuous production of neuroblasts is controlled by SVZ microenvironmental niche3,4. It is generally believed that enhancing neurogenic activities of endogenous NSCs may provide needed therapeutic options for disease states and after brain injury. However, SVZ NSCs can also differentiate into astrocytes. It remains unclear if there are conditions that favor astrogenesis over neurogenesis in the SVZ niche, and if astrocytes produced there exhibit different properties from others in the brain. We have uncovered that SVZ-generated astrocytes express high levels of Thrombospondin-4 (Thbs4)5,6, a secreted homopentameric glycoprotein, in contrast to cortical astrocytes which are Thbs4low. We found that localized photothrombotic/ischemic cortical injury initiates a marked increase in Thbs4hi astrocyte production from the postnatal SVZ niche. Tamoxifen-inducible nestin-CreERtm4 lineage-tracing demonstrated that it is these SVZ-generated Thbs4hi astrocytes, and not DCX+ neuroblasts, that home-in on the injured cortex. This robust post-injury astrogenic response required SVZ Notch activation, modulated by Thbs4 via direct Notch1 receptor binding and endocytosis to activate downstream signals, including increased Nfia transcription factor expression important for glia production7. Consequently, Thbs4KO/KO animals showed severe defects in cortical injury-induced SVZ astrogenesis, instead producing cells expressing DCX from SVZ to the injury sites. These alterations in cellular responses resulted in abnormal glial scar formation after injury, and significantly increased microvascular hemorrhage into the brain parenchyma of Thbs4KO/KO animals. Taken together, these findings have significant implications for post-injury applications of endogenous and transplanted NSCs in the therapeutic setting, as well as disease states where Thbs family members play important roles8,9.
Keywords: subventricular zone, astrogenesis, brain injury, Thbs4, Notch, tsp
We want to understand neurogenesis/astrogenesis choice in the postnatal SVZ niche, and the cellular properties of SVZ-generated astrocytes. CNS astrocytes secrete Thrombospondins (Thbs), a family of homotrimeric and homopentameric proteins6: we asked whether SVZ-generated astrocytes express different Thbs protein(s) than their cortical counterparts. We started by establishing primary SVZ adherent cultures from nestin-CreERtm4 (N4); rosa26reporter-tdTomato (RTM) animals, after postnatal day 7 (P7) tamoxifen injection. We showed previously that this N4 line can inducibly and efficiently lineage-trace progeny of postnatal/adult SVZ NSCs4,10 (Supplementary Fig. 1 and Mov. 1). Following 5 days of differentiation, tdTomato+ lineage-traced GFAP+ astrocytes showed strong immunohistochemical (IHC) staining for Thbs4 (Supplementary Fig. 2a). To confirm the specificity of this antibody staining, we performed the same culture experiment using Thbs4KO/KO mutant animals11, which revealed no Thbs4 immunofluorescence under identical experimental/imaging conditions (Supplementary Fig. 2b). Western blot analyses confirmed these findings (Supplementary Fig. 2c). Comparison of differentiated SVZ astrocyte cultures to primary astrocytes harvested from the cortex showed selective Thbs4 expression by SVZ astrocytes (Fig. 1a). This difference in Thbs4 expression was further demonstrated by quantitative PCR (qPCR) analyses of FACS-purified GFP+ cortical vs. SVZ astrocytes from GFAP-GFP transgenic animals (Fig. 1b). IHC staining on P14 brain sections indicated that Thbs4, while co-labeling with SVZ GFAP+ astrocytes, did not co-localize with Mash1+ transiently amplifying progenitors, DCX+ neuroblasts, or NG2+, Olig2+ populations in the SVZ niche (Supplementary Fig. 3a - e).
Figure 1
Figure 1
SVZ generation of Thbs4hi astrocytes
We next tested whether SVZ-generated GFAP+ astrocytes are fated to express Thbs4 in vivo. We transplanted second passage SVZ NSC cultures harvested from tamoxifen-induced N4; RTM animals into the cerebral cortex of WT/non-transgenic animals (Fig. 1c). Unlike transplantations into the SVZ, which generated neuroblasts that migrate to the olfactory bulb4,12 (Supplementary Fig. 4), tdTomato+ cells transplanted into the cortex after 2 to 4 weeks gave rise to GFAP+Thbs4hi astrocytes, contrasting with resident cortical astrocytes which were Thbs4low (Fig. 1c). Of the 402 N4 lineage-traced tdTomato+ cells counted over multiple experiments, 96.8% (389) showed GFAP expression. Strong Thbs4+ IHC co-staining was detected in 98.2% (382) of these GFAP+ cells.
Next, we wondered under which conditions the SVZ niche favored Thbs4hi astrocyte production. SVZ NSCs are thought to respond to middle cerebral artery occlusion-induced stroke by producing DCX+ neuroblasts that migrate into the striatum13. Although some have also reported gliogenic responses after injury14,15. To generate precisely localized cortical injuries directly over the SVZ niche we used photothrombosis, a well-defined ischemic injury model16 (Fig. 2a). We performed these injuries using N4; RTM animals after P6 tamoxifen injection: this timing allowed us to specifically target/lineage-trace SVZ NSCs, while minimizing Cre-reporter labeling of cortical cells10. We induced cortical injuries at P12 and examined the SVZ responses at 3 and 14 days post injury (dpi), using 3,3′-Diaminobenzidine (DAB) IHC staining against tdTomato, allowing simultaneous visualization of tdTomato-reporter expression and brain tissue histology. At 3 dpi, we did not see significant morphological changes to lineage-traced tdTomato+ cells around the SVZ (Fig. 2b). However, by 14 dpi, we observed robust populations of tdTomato+ cells between SVZ and cortical injury site (Fig. 2b). This delayed reaction was specific to SVZ/hemisphere ipsilateral to the injury, as we did not detect obvious changes to tdTomato+ cells in the contralateral cortex, nor did we see changes in the ipsilateral cortex in sham-treated control brains (Supplementary Fig. 5a, b). As a further control, we did not detect tdTomato+ cells in the injured cortex of N4; RTM animals without tamoxifen injection (Supplementary Fig. 5c). We also did not observe tdTomato+ cells next to superficial cortical injuries, suggesting a correlation between injury severity and SVZ responses (data not shown). All analyses were performed on cortical injuries that did not breach the corpus callosum (determined by sectioning through the entire injured area), limiting potential spill-over of SVZ niche neuroblasts into the injured areas.
Figure 2
Figure 2
Thbs4hi astrocyte production following photothrombotic cortical injury
IHC staining showed that the majority of tdTomato+ cells next to the injury site 14 dpi had complex morphologies, labeled strongly with anti-Thbs4 antibody, and co-stained with GFAP (Fig. 2c, d). Although we did not observe tdTomato+ cells at the injury site 3 dpi, Western blotting and IHC staining of SVZ tissue showed that, at this early time point, the ipsilateral SVZ had upregulated Thbs4 expression as compared to the contralateral side (Fig. 2e, f). This Thbs4 expression remained localized to GFAP+ astrocytes (Supplementary Fig. 3f). Repeating these injury experiments using the GFAP-Cre driver (JAX #004600) instead of N4, we observed similarly robust tdTomato+ lineage-traced cells around the injury site 14 dpi (Supplementary Fig. 6). Though they likely represents a heterogeneous cell population, since the GFAP-Cre driver also efficiently lineage-traced cortical cells (Supplementary Fig. 6). To investigate whether cortical astrocytes can upregulate Thbs4 expression to levels seen in SVZ astrocytes after injury, we performed qPCR analyses 3 dpi on FACS-sorted GFP+ cortical vs. SVZ astrocytes from GFAP-GFP animals (prior to significant migration from SVZ), which showed that SVZ astrocytes remained the Thbs4hi population (Supplementary Fig. 7).
What are the molecular signals controlling this injury-induced Thbs4hi astrogenesis from the SVZ? The Notch pathway is an important regulator of SVZ NSC and niche function10,17, as well as neurogenesis vs. gliogenesis choice18. To determine if Notch activation is required for Thbs4hi astrocyte production after cortical injury, we inducibly deleted RBPJκ19, the Notch Intra-Cellular Domain (NICD) co-transcriptional activator, using the N4 transgene. We crossed N4; RBPJκKO/+ mice to RTMFlox/Flox; RBPJκFlox/Flox mice and treated new mouse litters with tamoxifen at P6. We then compared lineage-traced tdTomato+ cells around the cortical injury site between N4; RTM; RBPJκFlox/+ (control) and N4; RTM; RBPJκKO/Flox inducible mutant (iKO) animals at 14 dpi. DAB staining revealed that while there were robust tdTomato+ cells between the SVZ and cortical injury site in the controls (Fig. 3a), this response was blunted in RBPJκ iKO animals (Fig. 3a, b). We next asked if increased Notch signaling can result in enhancement of SVZ response after injury. Using N4; RTM; rosa26r-NICDFlox/+ animals to over-express NICD in lineage-traced SVZ cells after tamoxifen injection, we repeated the cortical injury experiments. DAB staining 14 dpi showed significantly increased numbers of lineage-traced tdTomato+ cells at the injury site in NICD over-expressing animals (Fig. 3a, b). Consistent with these results, IHC staining of wild-type brain sections following cortical photothrombosis showed upregulated Notch1 receptor expression in the ipsilateral SVZ 2 dpi (Supplementary Fig. 8). And Western blot analyses 3 dpi revealed an increase in NICD protein in the ipsilateral SVZ (Fig. 3c).
Figure 3
Figure 3
Notch signaling and regulation of injury-induced SVZ astrogenesis
Ependymal cells, labeled/lineage-traced by FOXJ1-based reporters/drivers, have been reported to respond to ischemic injury by generating progeny that migrate to the injury site20. Since this N4 line also targets ependymal cells4,10, thus potentially lineage-tracing ependymal progeny after injury, we performed identical cortical injuries in FOXJ1-CreERt2; RTM animals after P6 tamoxifen injection. In repeated experiments we did not observe migration of tdTomato+ populations from SVZ to the cortical injury sites either early (3 dpi) or late (14 dpi) (Supplementary Fig. 9a and data not shown). The FOXJ1-CreERt2 driver also labeled mature cortical neurons, but this expression was independent from injury-induced cell proliferation (Supplementary Fig. 9a and data not shown). To rule out the possibility that modification of Notch signaling allowed ependymal cells to generate progeny responding to injury, we performed cortical injury experiments in RBPJκ iKO and rosa26r-NICD over-expression backgrounds using the FOXJ1-CreERt2 driver. In both genetic backgrounds we did not observe migration of tdTomato+ cells from SVZ to the injury sites (Supplementary Fig. 9b).
Thbs2 has been shown to physically interact with the Notch3 receptor in vitro21. Thus, we wondered if Thbs4 plays a direct role in modulating Notch activity after cortical injury. To test this, we first differentiated early passage SVZ NSC cultures in the presence of immobilized Jagged1-Fc. Since transient Notch activation is known to decrease neurogenesis18, immobilized Jagged1-Fc resulted in decreased neuroblast production compared to untreated control cultures (Fig. 3d, f). We repeated this assay with the addition of recombinant Thbs4 alone in the medium, and observed a similarly robust decrease in neuroblast production (Fig. 3d, f). This was confirmed by Western blot analyses for DCX protein after 5 days of differentiation (Fig. 3e, f). DAPT or DBZ, common Notch pathway inhibitors, conversely increased production of neuroblasts from differentiating SVZ cultures (Supplementary Fig. 10 and data not shown). Thbs4 was unable to blunt DAPT or DBZ-mediated effects (Supplementary Fig. 10), suggesting that Thbs4's function in this setting required Notch activity.
Since SVZ NSCs express the Notch1 receptor17, we asked whether Thbs4 and Notch1 can physically interact. Using varied concentrations of purified Thbs4 protein and recombinant Notch1-Fc fragment (including the first 13 extracellular EGF-like repeats of Notch1), pull-down experiments showed direct Thbs4/Notch1-Fc interactions in vitro (Supplementary Fig. 11a). mIgG2a, an isotype-specific control for Notch1-Fc, as well as purified Thbs2 protein, did not show Notch1-FC interactions (Supplementary Fig. 11a). We next harvested cellular extracts from primary SVZ NSC cultures with or without addition of Thbs4 in the medium. Immunoprecipitation (IP) with anti-Notch1 antibody was able to pull-down Thbs4 from the culture lysates in the +Thbs4 condition (Supplementary Fig. 11b). While under physiological conditions, IP from freshly isolated SVZ tissues using anti-Notch1 antibody did not detect significant Thbs4 pull-down (Supplementary Fig. 11c), similar IP experiments 3 dpi revealed Notch1/Thbs4 interactions (Fig. 3g).
Efficient Notch signaling requires receptor-endocytosis into endosomes22, and Thbs4 as a pentameric protein may promote Notch endocytosis and activation. To test this possibility, we cultured primary SVZ NSCs in the presence of both Thbs4 and late endocytosis blocker Dynasore. Addition of Thbs4 alone resulted in NICD upregulation, as detected by Western blotting 15 minutes after incubation, and lasting for several hours thereafter (Fig. 3h, Supplementary Fig. 11d). This NICD increase was blocked by Dynasore (Fig. 3h). By 36 hours after stimulation, Thbs4-induced NICD upregulation had subsided, and as expected with Dynasore added there was low NICD with or without Thbs4 in medium (Supplementary Fig. 11e). The transcription factor Nfia is an important regulator of gliogenesis downstream of Notch signaling7,23. Following Thbs4 addition during SVZ NSC differentiation in vitro, we detected increased Nfia expression over control conditions (Supplementary Fig. 11f). Similarly, Western blotting of SVZ tissues 3 dpi showed increased Nfia protein levels in the ipsilateral vs. contralateral SVZ (Fig. 3i), consistent with injury-induced SVZ astrogenic response (Fig. 2e, f).
Our findings raised the intriguing possibility that Thbs4, following cortical injury, is itself necessary for Notch-mediated SVZ astrogenesis. To test this, we first performed Western blot analyses on SVZ tissue from Thbs4KO/KO animals 3 dpi. While under physiological conditions we did not detect noticeable differences in SVZ NICD expression levels between Thbs4KO/+ (control) and Thbs4KO/KO mutant animals (Supplementary Fig. 12a), these mutants lacked NICD increase in the ipsilateral SVZ 3 dpi (Fig. 4a) unlike WT animals (Fig. 3c). Further, Thbs4KO/KO animals did not show appreciable increase in Nfia expression in the ipsilateral SVZ 3 dpi (Fig. 4a). We next tamoxifen-induced N4; RTM; Thbs4KO/KO animals to lineage-trace responding SVZ-derived cells after cortical injury, according to the same protocol described above. At 14 dpi, the tdTomato+ cells around the injury site showed a surprising neuroblast-like morphology, and mostly co-labeled with DCX rather than GFAP (Fig. 4b, c, Supplementary Fig. 12b). This is in striking contrast to cortical injuries in control animals, where few DCX+ cells were detected next to the injury site (SVZ neuroblast staining was used as internal control for DCX antibody, Fig. 4c, Supplementary Fig. 13). The observed mixture of tdTomato- and tdTomato+ DCX+ cells at the cortical injury site is consistent with the clonal nature of N4-mediated recombination following tamoxifen induction4,10.
Figure 4
Figure 4
SVZ astrogenesis defects in Thbs4 mutant mice after cortical injury
In preparing the injured brains from Thbs4KO/KO animals, we noticed significant hemorrhage around the injured cortical areas. We next performed brain magnetic resonance imaging (MRI) analyses on control and Thbs4KO/KO littermates. Using 3D structural MRI on brains inside intact skulls, we can identify the location and extent of cortical injuries (Supplementary Fig. 14a, b). In isotropic diffusion-weighted images, the boundaries of lesions were hyperintense in both control and Thbs4KO/KO animals (Supplementary Fig. 14a, b), demonstrating classical characteristics of stroke infarct24. The interiors of these lesions appeared hypointense as result of increased edema, and quantitative maps of diffusion coefficients confirmed hindered molecular diffusion in the infarcted, but faster diffusion in the edematous areas (Supplementary Fig. 14a, b). We did not detect significant Mean Diffusivity measurement differences between littermate control and Thbs4KO/KO animals in the infarcted or edematous cortical areas, either 2 dpi (data not shown) or 8 dpi (Fig. 4e, Supplementary Fig. 14d).
Iron in blood deoxyhemoglobin is paramagnetic, thus increasing tissue magnetic susceptibility in the presence of hemorrhage25. Using 3D spoiled-gradient-recalled (SPGR) sequence to measure magnetic properties, the edematous areas of Thbs4KO/KO animals showed both faster image-intensity decay, and faster R2* relaxation rate (rate of decay) as compared to littermate controls (Fig. 4d, Supplementary Fig. 14c). Thbs4KO/KO animals exhibited significantly increased areas of magnetic susceptibility in the injured cortex as compared to the uninjured contralateral side, while control animals showed only well-defined hyperintense boundaries surrounding the resolving cortical lesions (Fig. 4d, f, Supplementary Fig. 14c, e). While we did not detect these magnetic property differences early on at 2 dpi between control and Thbs4KO/KO animals (data not shown), the faster R2* rate and increased magnetic susceptibility in Thbs4KO/KO animals at the later time point indicated presence of extensive, unresolved hemorrhage in their injured cortical regions.
Cortical vasculature compromise can be detected by using biotinylated fixable dextran as tracer26. We perfused animals 7 dpi wisth biotinylated dextran and examined their injuries by fixed brain sections. GFAP antibody staining showed that while cortical glial scars can be readily identified in littermate controls, they were poorly defined in Thbs4KO/KO animals (Fig. 4g, Supplementary Fig. 12c). Furthermore, whereas biotinylated dextran was largely retained inside the vasculature adjacent to injured areas in littermate controls, in Thbs4KO/KO animals we detected widespread parenchymal biotinylated dextran next to the injury sites (Fig. 4g, h). These results are consistent with the MRI analyses above, and indicate continued microvascular bleeds after cortical injury.
Our findings revealed a surprising outcome where SVZ-mediated astrogenesis may be beneficial over neurogenesis in a period after cortical injury, in agreement with potentially protective roles for astrocytes during recovery process in the spinal cord27. Furthermore, we believe these results will have important implications for therapeutic interventions using transplanted and/or endogenous NSCs after brain injury28,29, as well as astrocytic tumors that can arise from the SVZ niche30.
Cell Culture
Adherent SVZ primary cultures were isolated and grown as described31. Cortical astrocyte cultures were grown as described32. Jagged1-Fc (R&D Systems) was plated at 5 μg/ml in PBS overnight to coat culture dish surfaces, followed by PBS washes. Recombinant Thbs4 (3 μg/ml, C. Eroglu), DAPT (5 μM, Tocris), DBZ (5 nM, Millipore) were freshly added to culture medium every other day during in vitro differentiation where indicated. Dynasore33 (Sigma) was used at 30 μM in culture medium.
Immunohistochemistry and live-imaging analyses
Preparation of brain tissue for immunohistochemistry (IHC) was as described10. For Thbs4 and DAB staining: after transcardiac perfusion, brains were removed, postfixed overnight, and cryoprotected in 30% sucrose at 4°C. 30 μm coronal sections were serially cut, and immediately incubated for 1 hr at room temperature (RT), floating in PBST blocking buffer containing 10% donkey serum. Primary antibody incubation was carried out at 4°C in blocking buffer overnight, followed by washes in PBST ×3, PBS alone ×3, and secondary antibody incubation in blocking buffer for 2 hrs at RT. DAB staining was carried out according to manufacturer instructions (Vectastain ABC Kit, Vector Labs). For cell counting and quantifications, IHC stained coronal sections, 90 μm apart, starting at the anterior portion of the anterior commissure through the septofimbrial nuclei, were analyzed and counted. Primary antibodies against the following antigens were used: Thbs4 (goat, 1:200, R&D Systems); GFP (chicken, 1:500, Aves Labs); RFP (rabbit, 1:1000, Rockland); GFAP (mouse, 1:2000, Sigma); Mash1 (mouse, 1:100, BD Biosci) DCX (guinea pig, 1:200, Millipore); NeuN (mouse, 1:500, Millipore); Notch1 (rabbit monoclonal EP1238Y, 1:500, Epitomics); Olig2 (rabbit, 1:800, Millipore); NG2 (mouse, 1:200, R&D Systems). Biotinylated fixable dextran (MW = 10 kDa, 1.0 mg/ml, Invitrogen) experiments and their image analyses were performed as described26. Live-imaging of migrating neuroblasts was performed as described34. All fluorescent images were acquired on Leica TCS SP5 confocal microscope, with control and experimental samples imaged under identical settings.
FACS sorting and gene expression analyses
Cortical and SVZ tissues from GFAP-GFP animals (JAX #003257) were dissected in warm NSC culture media31, dissociated in Neural Tissue Dissociation Kit (Miltenyi) according to manufacturer's protocol. Cell suspension was added to FACS tube on ice, sorted on BD FACS DiVa sorter, followed immediately by Trizol RNA extraction. 500 ng of total RNA was used for cDNA synthesis using SuperScript VILO cDNA Synthesis Kit (Invitrogen). Quantitative PCR analyses were performed as described35, using the following DNA primers: Thbs4 F: 5′-atccctgctatccaggtgtg-3′, R: 5′-ggcagctcctttcagtcttg-3′; Nfia F: 5′-ccagccagccaagtgaag-3′, R: 5′-gctcagtcacactgaaaacacc-3′; housekeeping gene controls GAPDH F: 5′-catggccttccgtgttcct-3′, R: 5′- tgatgtcatcatacttggcaggtt-3′, and PPIA F: 5′-cgagctctgagcactggag-3′, R: 5′-gatgccaggacctgtatgct-3′. Consistent results were obtained using either housekeeping primer sets.
SDS-PAGE and immunoblotting
Protein extract preparation and Western blotting were performed as described4. NIH ImageJ software was used for quantification analyses. Primary antibodies against the following antigens were used: Thbs4 (goat, 1:500, R&D Systems); Thbs2 (mouse, 1:500, Millipore); DCX (guinea pig, 1:1000, Millipore); NICD/Notch1 (rabbit EP1238Y, 1:1000, Millipore); Nfia (rabbit, 1:2000, Active Motif); actin (mouse, 1:5000, Abcam). For pull-down experiments, purified recombinant Thbs4 or Thbs2 (R&D Systems) was incubated for 1 hr at 37°C with either 200 ng mouse Notch1-FC chimera (R&D Systems, 5267-TK) or mouse IgG2a isotype control (Abcam) in Dulbecco's PBS + 1% BSA, 0.1% Triton X-100. Protein G-coupled DynaBeads (Invitrogen), pre-blocked in DPBS + 3% BSA, were then added for 10 min at 37°C, followed by 5 washes in DPBS + 0.1% Triton X-100, and analyzed by Western blotting. For cultured cells, media with or without Thbs4 (3 μg/mL) were first added for 4 hours, washed 2 times with cold PBS, followed by addition of lysis buffer (50mM Tris pH 8.0, 75mM NaCl, 1mM EDTA, 5% sucrose, 0.25% Triton x-100, mini-complete protease inhibitor cocktail), sonication, and centrifuged for 10 minutes at 4°C. Lysates were pre-cleared with Protein A agarose beads (Roche). Rabbit anti-Notch1 antibody (5 μg, Millipore EP1238Y) was added to 1 ml of lysate and incubated overnight at 4°C, followed by addition of Protein A agarose beads, washes as described above, and Western blotting analysis. SVZ IP experiments were performed as described10 with following modifications: CHAPS lysis buffer contained 5mM CHAPS, 50 mM Tris (pH 7.4), 150 mM NaCl, 1 mM CaCl, 5% sucrose, 0.5% Triton X-100, protease inhibitor cocktail (Roche) + sodium orthovanadate. Supernatants after lysis were subject to two rounds of pre-clearing with BSA-blocked Protein G agarose beads (Roche) for 1 hr each, followed by incubation with rabbit anti-Notch1 antibody (Millipore EP1238Y) for 1 hr, and overnight incubation with BSA-blocked Protein G agarose beads, all at 4°C. Beads were washed five times in lysis buffer, three times in PBS prior to suspension in sample buffer for Western blotting.
Cortical injury and in vivo injections
Photothrombosis cortical injury was performed as described36. Briefly, animals were anesthetized and body temperature maintained at 37°C with recirculating water heating pad. Saline solution of rose bengal photosensitive dye (10 mg/ml in saline, 0.1 mg per gram of body weight) was delivered intraperitoneally. Midline scalp incision was made to expose the skull. As external light source, Zeiss KL 1500 LCD (light intensity at 5, 6-minute duration) with 2.5 mm opening light guide was used to induce photothrombosis. Transplantation of passage 2 primary adherent SVZ culture was performed as described4. 13 out of 37 transplanted animals showed successfully grafted tdTomato+ cells on analyses. Tamoxifen (10 mg/ml, freshly dissolved in corn oil) was injected intraperitoneally at 0.15 mg per gram of body weight to induce CreER-mediated recombination. All mouse experiments were performed according to approved protocol by IACUC at Duke University.
Magnetic resonance imaging and analyses
Pairs of injured Thbs4KO/+ and Thbs4KO/KO mice were scanned on 9.4 Tesla (400 MHz) 89-mm vertical bore MRI scanner (Oxford Instruments) with shielded coil providing gradients of 2200 mT/m. Mice were perfused with 10% buffered formalin as previously described37, followed by overnight fixation in formalin and 3 day incubation in PBS before imaging. All brains were kept within the cranium to prevent potential damage by removal. Diffusion-weighted images (DWI) were acquired using 3D spin-echo sequence with following parameters: field of view (FOV) = 22×11×11 mm3, matrix = 164×82×82, TE = 12 ms, TR = 2500 ms. One image volume was acquired without diffusion weighting, and diffusion weighting was achieved by applying two half-sine gradient pulses around the 180° refocusing pulse. To produce isotropic weighting, six non-collinear diffusion encoding directions were used at b-value = 3000 s/mm2. A diffusion tensor was fitted using seven image volumes and mean diffusivity was calculated as described38. To examine intracranial hemorrhage, brains were scanned using 8-echo 3D spoiled-gradient-recalled (SPGR) sequence with the following parameters: FOV = 22×11×11 mm3, matrix = 512×256×256, initial TE = 4.4 ms, echo spacing = 4.9 ms, TR = 100 ms, flip angle = 45°. R2* relaxation rate was fitted with exponential decay curve. Tissue magnetic susceptibility was quantified as described39. Regions of infarct and edema were segmented out based on Mean Diffusivity maps generated via FSL software (Oxford University), and comparable regions in the contralateral uninjured cortex were drawn as references. For each region, Mean Diffusivity, R2* relaxation rate, and Magnetic Susceptibility were measured. Similar results were obtained with addition of MRI contrast agent ProHance (Bracco Diagnostics, Princeton, NJ) to formalin fixation (1:9, v:v).
Supplementary Material
Acknowledgments
We thank Doug Melton for rosa26r-NICD mice; Tasuku Honjo for RBPJκ-flox mice; Fan Wang for rosa26r-tdTomato mice; Emma Rawlins for FOXJ1-CreERt2 mice; Ben Deneen, Sandeep Singh for helpful discussions; Gray Lyons, Ryan Andersen, Peer Heine, Dawn Fromme, and Sam Collins for project assistance; Duke Flow Cytometry Facility for help with FACS; Wei Li and Duke Center for In Vivo Microscopy/Brain Imaging for MRI analyses; Terry Lechler, Anne West, and Brigid Hogan for helpful comments on manuscript. This work was supported by National Biomedical Technology Resource Center Grant P41 RR005959 (C.L.); George & Jean Brumley Endowment, Sontag Foundation, David & Lucile Packard Foundation, March of Dimes, and N.I.H. Director's New Innovator Award 1 DP2 OD004453-01 (C.T.K.).
Footnotes
Author Contributions: E.J.B. performed injury and biochemical experiments; D.L. performed gene expression and live-imaging experiments; K.A. performed in vivo IP experiments; P.P.-G. performed SVZ staining and analyses; R.J., H.S., D.W. assisted with injuries and their analyses; C.L. performed MRI scanning and analyses; C.E. provided reagents and experimental insight; C.T.K. performed transplantations and conceived the project. E.J.B., D.L., R.J. assembled figures and C.T.K. wrote the paper. All authors discussed results and commented on the manuscript.
Author Information: Reprints and permissions information is available at www.nature.com/reprints.
The authors declare no competing financial interests.
Supplementary Information is available in the online version of the paper.
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