Modeling CADASIL vascular pathologies with patient-derived induced pluripotent stem cells
- 814 Downloads
Cerebral autosomal dominant arteriopathy with subcortical infarcts and leukoencephalopathy (CADASIL) is a rare hereditary cerebrovascular disease caused by a NOTCH3 mutation. However, the underlying cellular and molecular mechanisms remain unidentified. Here, we generated non-integrative induced pluripotent stem cells (iPSCs) from fibroblasts of a CADASIL patient harboring a heterozygous NOTCH3 mutation (c.3226C>T, p.R1076C). Vascular smooth muscle cells (VSMCs) differentiated from CADASIL-specific iPSCs showed gene expression changes associated with disease phenotypes, including activation of the NOTCH and NF-κB signaling pathway, cytoskeleton disorganization, and excessive cell proliferation. In comparison, these abnormalities were not observed in vascular endothelial cells (VECs) derived from the patient’s iPSCs. Importantly, the abnormal upregulation of NF-κB target genes in CADASIL VSMCs was diminished by a NOTCH pathway inhibitor, providing a potential therapeutic strategy for CADASIL. Overall, using this iPSC-based disease model, our study identified clues for studying the pathogenic mechanisms of CADASIL and developing treatment strategies for this disease.
KeywordsCADASIL iPSC NOTCH NF-κB vascular smooth muscle
Cerebral autosomal dominant arteriopathy with subcortical infarcts and leukoencephalopathy (CADASIL), a hereditary cerebrovascular disease caused by a NOTCH3 gene mutation (Joutel et al., 1996; Goate and Morris, 1997; Rutten et al., 2014), has the clinical manifestations of recurrent ischemic stroke, progressive cognitive decline and mental disorders (Wang et al., 2011; Di Donato et al., 2017; Fang et al., 2017). The average age at onset for CADASIL is approximately 40 years, which is younger than that of many other non-hereditary cerebrovascular diseases (Herve and Chabriat, 2010; Wang, 2018). Due to early onset and the lack of effective therapy, CADASIL patients face a serious risk of poor quality of life and eventually death.
Blood vessel walls are composed of three layers: the tunica intima, tunica media and tunica adventitia. The tunica intima mainly consists of vascular endothelial cells (VECs) and connective tissues. The structure of the tunica media varies in different vessels, with abundant parallel elastic fibers and vascular smooth muscle cells (VSMCs) in large and medium arteries but mainly VSMCs in small arteries and veins (Swift and Weinstein, 2009; Krings et al., 2011). NOTCH3 is predominantly expressed in the vascular system and is particularly important for the maturation of VSMCs (Villa et al., 2001; Domenga et al., 2004; Liu et al., 2010; Jin et al., 2014; Granata et al., 2015; Gatti et al., 2018). Consistent with the tissue localization and function of NOTCH3, CADASIL mainly affects VSMCs in the tunica media. The specific pathological feature of CADASIL is the deposition of granular osmiophilic material (GOM) on the basement membrane of VSMCs, which is accompanied by prominent thickening of vessel walls due to the deposition of various extracellular matrix proteins (Tikka et al., 2009; Dong et al., 2012; Monet-Lepretre et al., 2013; Zhang et al., 2015b; Capone et al., 2016). Abnormalities in proliferation ability, mitochondrial function and cytoskeleton structure have also been identified in VSMCs from CADASIL patients and mice (Domenga et al., 2004; Tikka et al., 2012; Viitanen et al., 2013; Panahi et al., 2018). Despite these prior studies, detailed phenotypic profiles of VSMCs and other types of cells in CADASIL patients, such as VECs, and the underlying mechanism of CADASIL remain elusive.
Study of the pathogenesis of CADASIL is limited, largely due to a lack of appropriate experimental models. CADASIL mouse models have been used to study CADASIL-specific GOM deposits and vascular dysfunction (Shibata et al., 2004; Lacombe et al., 2005; Joutel et al., 2010). However, such mice are mostly transgenic animals that overexpress mutant human or rodent NOTCH3 and thus have different genotypes than CADASIL patients (Joutel, 2011). Immortalized primary VSMCs derived from CADASIL patients have transformation-related artifacts and are difficult to obtain due to the rarity of CADASIL. Thus, a model that not only faithfully represents disease-associated defects but also is applicable for patients is urgently needed. In recent years, the development of somatic cell reprogramming and in vitro directed differentiation techniques have provided effective approaches for modeling disease-specific phenotypes, conducting pathogenesis research and performing drug screening (Li et al., 2011; Liu et al., 2011a, b, 2012, 2014; Fu et al., 2016; Li and Izpisua Belmonte, 2016; Wang et al., 2017).
Here, we generated a non-integrative iPSC-based disease model for CADASIL and obtained CADASIL-specific VSMCs and VECs. In CADASIL VSMCs, phenotype-associated aberrant transcripts and disease-associated cellular dysfunction, including NOTCH and NF-κB pathway activation, cytoskeleton disorganization, and elevated cell proliferation, were identified. Treatment with a NOTCH pathway inhibitor alleviated the upregulation of NF-κB target genes in CADASIL VSMCs, suggesting a potential pharmacological intervention strategy for CADASIL. Overall, we established an iPSC-based disease model for CADASIL and thereby provided valuable clues for pathogenic analysis and therapeutic strategy development.
Generation of CADASIL-specific non-integrative iPSCs
Transcriptional profile changes in CADASIL VSMCs
Activation of NF-κB in CADASIL VSMCs was related to NOTCH pathway upregulation
CADASIL VSMCs exhibited hyperproliferation and abnormal cytoskeleton structure
Transcriptional changes associated with NOTCH and NF-κB signaling pathway, or the cytoskeleton in CADASIL VSMCs were not detectable in CADASIL VECs
We then performed RNA sequencing to determine whether CADASIL VECs had disease-specific transcriptomic changes. The high correlation coefficients between replicates confirmed high reproducibility (Fig. 5G). In total, 379 upregulated genes and 330 downregulated genes were identified in CADASIL VECs (Fig. 5H and 5I), which had fewer differentially expressed genes than CADASIL VSMCs. GSEA and GO-BP analyses revealed that cell-cell adhesion via adhesion molecules and innate immune response were enriched in CADASIL VECs (Fig. 5J and 5K). However, the upregulated genes in CADASIL VSMCs that were associated with the NOTCH signaling pathway, the NF-κB signaling pathway, or the cytoskeleton were not upregulated in CADASIL VECs, suggesting that changes in transcriptional levels of these genes were specific to VSMCs. Upregulated genes in CADASIL VECs were verified by RT-qPCR (Fig. S2A), and downregulated genes in these cells were also verified by GO-BP analysis and RT-qPCR (Fig. S2B and S2C). Taken together, our findings showed that we generated CADASIL-specific VECs, but transcriptional profiling changes associated with the NOTCH signaling pathway, the NF-κB signaling pathway, or the cytoskeleton observed in CADASIL VSMCs were not detected in CADASIL VECs.
Disease-associated phenotypes observed in CADASIL VSMCs were not detected in CADASIL VECs
CADASIL VSMCs and VECs were more sensitive to inflammatory stimuli
Increased inflammation and vessel wall remodeling have been widely reported in diverse angiopathies, such as atherosclerosis, diabetes angiopathy, and hypertension angiopathy (Brand et al., 1996; Lontchi-Yimagou et al., 2013; Dinh et al., 2014; Viola and Soehnlein, 2015). In addition, vessel wall remodeling, as manifested by extracellular matrix protein deposition in the VSMC basement membrane and on vessel walls, has been implicated in CADASIL (Dong et al., 2012; Monet-Lepretre et al., 2013; Zhang et al., 2015b; Capone et al., 2016). This possibility is consistent with the upregulation of genes encoding various collagens in our CADASIL VSMCs, which was demonstrated via RNA sequencing analysis. The NF-κB pathway plays an important role in the inflammatory response. Upon stimulation, activated NF-κB translocates into the nucleus to promote the expression of genes encoding cytokines, chemokines and adhesion molecules as well as genes involved in extracellular matrix remodeling. Upregulation of these genes leads to increased vascular inflammation and vascular wall reconstruction, eventually resulting in vascular dysfunction (Baker et al., 2011; Killeen et al., 2014; Wang et al., 2018a). However, it remains unclear whether the NF-κB pathway contributes to CADASIL angiopathy. In our study, transcriptomic data showed that NF-κB target genes associated with vascular inflammation and vessel wall remodeling, including THBS1, MMP1, ADAM19 and TNFSF15 (Bonnefoy et al., 2008; Edwards et al., 2008; Kim et al., 2008; Bin et al., 2009; Penn et al., 2014), were upregulated in CADASIL-specific VSMCs. Among these genes, THBS1 encodes thrombospondin-1 (TSP1), which has been implicated in vascular dysfunction in pulmonary hypertension and various cerebrovascular diseases (Krishna and Golledge, 2013; Rogers et al., 2017), and MMP1 (which encodes a matrix metalloprotease) has been shown to promote the occurrence of hypertension, atherosclerosis and thrombosis (Dollery and Libby, 2006; Trivedi et al., 2009; Agrinier et al., 2013). Therefore, the upregulation of NF-κB target genes in CADASIL VSMCs may contribute to CADASIL-associated vascular dysfunction due to vessel wall remodeling and vascular inflammation. In addition, we found a more significant up-regulation of downstream genes of NF-κB in CADASIL VSMCs and VECs under TNFα-induced inflammatory condition. The observed excessive sensitivity to inflammatory stimuli of the CADASIL VSMCs and VECs suggests that CADASIL patients may suffer from cerebral blood vessels overly susceptible to injury under inflammatory conditions, aggravating the progression of angiopathy.
Our study indicates that the R1076C (c.3226C>T) NOTCH3 mutation may be linked to the activation of NOTCH signaling, at least in human VSMCs. This particular mutation is located within the exon 20 encoding the 27-28 EGFr domain of NOTCH3 (Joutel et al., 1997; Rutten et al., 2016), leading to the addition of a seventh cysteine residue as seen in many typical CADASIL mutations. Upregulation of NOTCH pathway was often associated with cysteine-related pathogenic mutations (Donahue and Kosik, 2004; Haritunians et al., 2005; Baron-Menguy et al., 2017), but how these mutations mediate the activation of NOTCH pathway and occurrence of CADASIL angiopathy remain unclear. One possible explanation is that these mutations interrupt the pairing of the disulfide bond in EGFr domain of NOTCH3 (Rutten et al., 2016). Subsequently, the unpaired cysteine residue causes the self-aggregation of the mutant protein, which inhibits the clearance of NOTCH3 and may enhance NOTCH pathway (Takahashi et al., 2010; Duering et al., 2011; Meng et al., 2012). The NOTCH pathway is evolutionarily conserved and implicated in the regulation of embryonic and organism development in many cell types at various stages (Penton et al., 2012; Andersson and Lendahl, 2014b; Bray, 2016; Siebel and Lendahl, 2017). Canonically, after binding to ligands, the NOTCH intracellular domain (NICD) translocates into the nucleus to promote the expression of downstream genes, mainly hairy and enhancer of split (HES) and HES-related with YRPW motif (HEY) genes. Moreover, a non-canonical branch of NOTCH signaling involves interaction with other signaling pathways, including the NF-κB pathway (Kopan and Ilagan, 2009; Andersson et al., 2011; Andersen et al., 2012; Guruharsha et al., 2012; Andersson and Lendahl, 2014a; Ayaz and Osborne, 2014). Multiple studies have shown that activation of the NOTCH pathway upregulates the NF-κB pathway (Vacca et al., 2006; Shin et al., 2014; Ruan et al., 2016), partially due to interaction between the NICD and NF-κB that prolongs retention of NF-κB in the nucleus (Shin et al., 2006). Consistent with the prior findings, we found that the activation of NF-κB pathway in CADASIL VSMCs was associated with the upregulation of NOTCH signaling and that the NOTCH pathway inhibitor DAPT partially alleviated the expression of NF-κB target genes, providing a new mechanism of and a potential therapeutic target for CADASIL angiopathy.
The causal relationship between NOTCH activation and VSMC proliferation has been implicated in multiple studies (Sweeney et al., 2004; Song et al., 2015; Wu et al., 2016), and abnormal VSMC proliferation is frequently related to and a contributor to pathological processes such as neointima formation and vascular remodeling (Rudijanto, 2007; Chistiakov et al., 2015; Lyon et al., 2016). In our study, both NOTCH activation and increased proliferation ability were observed in CADASIL VSMCs; thus, NOTCH activation may be a factor that contributes to CADASIL angiopathy.
In CADASIL patients and mice, cerebral vessels exhibit reduced response to intraluminal pressure changes and drug stimulation (Chabriat et al., 2000; Pfefferkorn et al., 2001; Joutel et al., 2010; Moreton et al., 2017). In our study, we found abnormalities in the structure of vimentin, a major component of intermediate filaments, in CADASIL VSMCs. NF-κB has been found to positively regulate transcriptional levels of vimentin (Chen et al., 1996; Xu et al., 2016). Accordingly, changes in vimentin structure in our CADASIL VSMCs may be induced by NF-κB activation. We also found abnormal microfilament structure in CADASIL VSMCs, which was consistent with findings from previous studies of CADASIL mice and primary VSMCs from patients (Domenga et al., 2004; Tikka et al., 2012). The NOTCH pathway has been reported to promote the expression of smooth muscle α-actin and the activity of Rho kinase (Noseda et al., 2006; Venkatesh et al., 2011), which may contribute to microfilament disorganization, thereby affecting dynamic regulation of the actin filament structure. In vascular cells, the cytoskeleton not only plays an important role in maintaining tissue and cell morphology and function (Fletcher and Mullins, 2010; Kassianidou and Kumar, 2015) but also helps to sense changes in luminal blood flow and assists with vasoconstriction and vasorelaxation (Henrion et al., 1997; Yamin and Morgan, 2012). We therefore speculated that the abnormal cytoskeleton structure in CADASIL VSMCs may contribute to disease-associated aberrant vasomotor function.
We established CADASIL VECs for the first time, permitting the study of cell type-specific effects of CADASIL in VSMCs and VECs in parallel. Almost none of the changes in cellular phenotypes or gene expression profile observed in CADASIL VSMCs manifested in our CADASIL VECs, suggesting that the relevant NOTCH3 gene mutation (c.3226C>T, p.R1076C) produces a cell type-specific effect. Notably, VEC abnormalities have been reported in the skin tissues of CADASIL patients, and electron microscopic observations of such tissues have revealed intracytoplasmic vacuoles, cell shrinkage, and extracellular collagen deposition (Ruchoux et al., 1994; Ruchoux and Maurage, 1998). However, it was unclear whether these changes reflect primary abnormalities of VECs or are secondary to vessel wall structural damage or aberrant cell-cell communication. Our transcriptome data reveal some abnormalities in CADASIL VECs, such as changes in innate immunity and cell-cell adhesion. We also observed the upregulation of downstream genes of NF-κB in CADASIL VECs under TNFα-induced inflammatory condition, suggesting that the VECs may contribute to CADASIL angiopathy in the presence of external inflammatory stimuli. It is worth noting that the transcriptomic profiles of in vitro cells might also be partially affected by changes in the microenvironment. Thus, the detailed cellular phenotypes and underlying mechanisms awaits further exploration.
Vessel wall is comprised of three layers. Except for the VECs in the intima and the VSMCs in the media, fibroblasts and mesenchymal stem cells (MSCs) in the adventitia also play an important role in vascular-associated diseases (Swift and Weinstein, 2009; Krings et al., 2011; Wang et al., 2018a). However, the role of NOTCH pathway in perivascular MSCs remains unclear. Our preliminary data suggest that CADASIL iPSC-derived MSCs may undergo premature aging (data not shown), which may contribute to depletion of perivascular MSCs in CADASIL. Thus the abnormalities of CADASIL MSCs likely reflect the previously reported changes of pericytes in CADASIL (Gu et al., 2012; Craggs et al., 2015; Ghosh et al., 2015).
CADASIL being a rare disease, only one patient was involved in our study. Despite that we used two WTs, isogenic disease-free control line may be even more helpful to establish in the future for the better simulation of disease phenotypes and understanding of underlying mechanisms (Li et al., 2011; Liu et al., 2011b; Wang et al., 2017). At the same time, many studies have pointed out that gene-corrected isogenic iPSCs have a good application prospect in the treatment of many diseases, such as the repair of damaged cardiovascular systems using iPSC-derived vascular cells (Ye et al., 2014; Jung et al., 2017; Zhang et al., 2018a). Therefore, generation of gene-corrected isogenic iPSCs may also help searching therapeutic maneuvers for CADASIL.
In summary, we have modeled CADASIL-related vascular pathologies using an iPSC-based disease model and generated corresponding VSMCs and VECs for phenotypic and mechanistic studies. Our study not only unearthed novel disease-associated cellular phenotypes and gene expression changes, thereby generating clues for future pathogenesis research, but also provided potential therapeutic strategies for CADASIL.
Materials and methods
Human fibroblasts were cultured in high glucose DMEM (Invitrogen) supplemented with 10% FBS (Gemcell), 0.1 mmol/L non-essential amino acids (NEAA, Gibco), 2 mmol/L GlutaMAX (Gibco) and 1% penicillin/streptomycin (Invitrogen). Human iPSCs were maintained on mitomycin C-inactivated mouse embryonic fibroblast (MEF) feeder in human ESC culture medium containing 80% DMEM/F12 (Gibco), 20% Knockout Serum Replacement (Gibco), 0.1 mmol/L NEAA (Gibco), 2 mmol/L GlutaMAX (Gibco), 55 μmol/L β-mercaptoethanol (Invitrogen) and 10 ng/mL FGF2 (Joint Protein Central) or on Matrigel (BD Biosciences) in mTeSR medium (STEMCELL Technologies). Human VSMCs were cultured in N2B27 medium (Wang et al., 2018a) supplemented with 10 ng/mL PDGF-BB (Peprotech). Human VECs were cultured in EGM-2 medium (Lonza).
Non-integrative iPSCs generation
Fibroblasts were cultured from the skin of a CADASIL patient harboring a heterozygous NOTCH3 mutation (c.3226C>T, p.R1076C) and two healthy controls. Primers for identification of the heterozygous NOTCH3 mutation: NOTCH3 forward primer, CACGTACCTCCTGCTAGTGTGAGCCGAA, NOTCH3 reverse primer, AGGCTGAAGCAGAAGAATCACCTGAACCC. The study was approved by the ethics committee of the Peking University First Hospital and a written informed consent was obtained. iPSCs were generated by electroporating fibroblasts with episomal vectors including pCXLE-hOCT3/4-shp53-F, pCXLE-hSK and pCXLE-hUL as previously described (Li et al., 2011; Okita et al., 2011; Liu et al., 2014; Fu et al., 2016; Wang et al., 2017). The generated iPSCs were manually picked and maintained on MEF feeder.
RT-PCR and RT-qPCR
Total RNA extraction and cDNA synthesis were performed using TRIzol reagent (Invitrogen) and GoScript Reverse Transcription System (Promega). For RT-PCR, cDNA was applied to PCR using primers including: GAPDH forward primer, TCGGAGTCAACGGATTTGGT, GAPDH reverse primer, TTGCCATGGGTGGAATCATA. NANOG forward primer, ACAACTGGCCGAAGAATAGCA, NANOG reverse primer, GGTTCCCAGTCGGGTTCAC. OCT4 forward primer, GGGTTTTTGGGATTAAGTTCTTCA, OCT4 reverse primer, GCCCCCACCCTTTGTGTT. SOX2 forward primer, CAAAAATGGCCATGCAGGTT, SOX2 reverse primer, AGTTGGGATCGAACAAAAGCTATT. RT-qPCR was carried out with SYBR Green PCR Master Mix (Bio-Rad) on a CFX-384 RT-qPCR system (Bio-Rad). The relative expression of genes was normalized by 18S rRNA transcript. Primers used for RT-qPCR are listed in Table S1.
Briefly, 5 × 106 iPSCs per line were injected subcutaneously into NOD/SCID mice (male, 6–8 weeks). About three months after injection mice were killed and teratomas were accessed for immunofluorescence. All murine experiments were conducted with the approval by the Institute of Biophysics, Chinese Academy of Science.
Bisulfite sequencing of the OCT4 promoter
Genomic DNA was extracted with Qiagen Blood and Tissue kit. Bisulfite modification of genomic DNA was carried out using CpGenome Fast DNA Modification Kit (Millipore) following the manufacturer’s instructions. The modified genomic fragment of OCT4 promoter was amplified using LA Taq Hot StartVersion (TAKARA) as previously described (Duan et al., 2015). The PCR products were then purified using PCR purification kit (Qiagen) and subsequently cloned into the pMD20 T vector (TAKARA). Seven clones from each sample were sequenced. Primers used for PCR: me-OCT4 forward primer, ATTTGTTTTTTGGGTAGTTAAAGGT, me-OCT4 reverse primer, CCAACTATCTTCATCTTAATAACATCC.
Cell cycle analysis
For cell cycle analysis, 1 × 106 cells were collected and fixed in 75% ice-cold ethanol at −20 °C overnight. The cells were then washed twice with PBS and stained with 0.02 mg/mL propidium iodide and 0.2 mg/mL RNase at 37 °C for 30 min. Cells were examined using a flow cytometry (BD LSRFortesa) and cell-cycle phase distributions were analyzed by ModFit software (Wang et al., 2018b).
Clonal expansion assay
The single-cell clonal expansion assay was carried out as previously described (Wu et al., 2018). Briefly, 2,000 cells were seeded onto 12-well plate and each line was analyzed in triplicate. The cell density was analyzed by ImageJ2x 669 184.108.40.206 software after crystal violet staining.
Generation of VSMCs
VSMC differentiation was carried out as previously described (Patsch et al., 2015). Briefly, iPSCs were unicellularized using TrypLE Express (Gibco) and seeded onto matrigel-coated 6-well plates at a density of 3 × 105 per well. After incubated in mTeSR supplemented with 10 µmol/L Y-27632 (Selleck) for one day, cells were then cultured in the N2B27 medium supplemented with 25 ng/mL BMP4 (R&D) and 8 μmol/L CHIR99021 (Selleck) for 3 days. Finally, cells were cultured in N2B27 medium supplemented with 10 ng/mL PDGF-BB (Peprotech) and 2 ng/mL Activin A (HumanZyme) for another 2 days and sorted after stained with anti-human CD140b-PE (BD biosciences, 558821, 1:200) by a flow cytometry (BD FACSAria IIIu). IgG-PE (BD biosciences, 555749) was used as an isotype control.
Generation of VECs
The iPSC clones were picked onto matrigel-coated 6-well plates in mTeSR medium. The next day culture medium was changed to EGM-2 medium (Lonza) supplemented with 25 ng/mL BMP4 (R&D), 3 µmol/L CHIR99021 (Selleck), 3 µmol/L IWP2 (Selleck) and 4 ng/mL FGF2 (Joint Protein Central) for 3 days. The cells were then cultured in EGM-2 medium supplemented with 50 ng/mL VEGF (HumanZyme), 10 ng/mL IL6 (Peprotech) and 20 ng/mL FGF2 (Joint Protein Central) for another 3 days. VECs were stained with anti-human CD34-FITC (BD biosciences, 555821, 1:200), anti-human CD201-PE (BD Biosciences, 557950, 1:200), and anti-human CD144-APC (BD Biosciences 561567, 1:200) and then sorted by a flow cytometry (BD FACSAria IIIu). IgG-FITC (BD biosciences, 555748), IgG-PE (BD biosciences, 555749) and IgG-APC (BD Biosciences, 555751) were used as isotype controls (Yang et al., 2017).
Identification of VEC surface markers
5 × 105 cells were collected and stained with anti-human CD31-FITC (BD biosciences, 557508, 1:100) and anti-human CD144-PE (BD Biosciences 561714, 1:200) and analyzed by a flow cytometry (BD FACSAria IIIu). IgG-FITC (BD biosciences, 555748) and IgG-PE (BD biosciences, 555749) were used as isotype controls.
Measurement of nitric oxide (NO)
About 5 × 105 VECs were treated with DAF-FM (Molecular Probes) to detect intracellular NO according to the manufacturer’s instructions. After stained for 30 min at room temperature, cells were quantified by a flow cytometry (BD FACSAria IIIu). The average fluorescence intensities were analyzed by FlowJo_V10 software.
Dil-Ac-LDL uptake assay
In brief, ECs were incubated with Dil-Ac-LDL (Molecular Probes) in EC culture medium for 6 h. For FACS analysis, cells were collected and analyzed by a flow cytometry (BD FACSAria IIIu). The average fluorescence intensities were analyzed by FlowJo_V10 software.
In vitro tube formation assay
Briefly, 6.5 × 104 VECs were suspended in 500 μL medium and then seeded on matrigel-coated 24 well plates. After cells were incubated for 8 h at 37 °C, formed tube-like structures were stained with Calcein-AM (Invitrogen) and visualized by fluorescence microscope (Olympus).
Transwell migration assay
Briefly, 2 × 104 cells were seeded on top of the 0.8 μm filters of Boyden chambers (Millipore) in serum deprivation medium. Then the filters were placed into 24 culture plate wells containing normal culture medium. Cells were allowed to migrate for 24 h in a humidified incubator at 37 °C, and 3 replicates were performed for each line. After incubation, the filter inserts were fixed with 4% paraformaldehyde and then the migrated cells were stained by purple crystal 30 min at room temperature. After washing 3 times using PBS, photograph was taken using light microscope and the number of migrated cells was counted with ImageJ2x 669 220.127.116.11.
Monocyte adhesion assay
Monocyte adhesion assay was carried out as previously described (Wang et al., 2018a). Briefly, 2 × 105 VECs were seeded in each well of 12-well plate. The next day, VECs were treated with or without 10 ng/mL TNFα (Peprotech) for 12 h. Then, 2 × 106 monocytes were co-cultured with VECs for 2 h after stained with Calcein-AM (Invitrogen). The monocytes adhered on endothelium were visualized by fluorescence microscope (Olympus) after rinsed by PBS for 5 times carefully. The number of adhered monocytes was analyzed by ImageJ2x 669 18.104.22.168 software.
Cells cultured in equal volume of medium were treated with or without 10 ng/mL TNFα (Peprotech) for 12 h. The cell culture medium was collected and filtered to remove cell debris, and the cell number was calculated at the same time. Concentration of secreted IL6 in the culture medium of cells was detected using Biolegend’s ELISA kit (Cat. No. 430504) following the manufacturer’s instructions, and 4–6 replicates were performed for each sample. The final concentration was obtained by normalization according to the number of cells and was recorded as pg/mL per 104 cells.
About 1 × 106 cells were lysed with 100 μL RIPA buffer [50 mmol/L Tris-HCl (pH = 7.5), 150 mmol/L NaCl, 1% NP-40, 0.5% sodium deoxycholate, 0.1% SDS] supplemented with NaF, NaVO4 and a protease-inhibitor mixture (Roche). Typically 20 µg of protein were separated by SDS-PAGE and then transferred to a PVDF membrane (Millipore). After blocked with 5% skimmed milk powder, the membrane was incubated with primary antibody overnight at 4 °C and then with HRP-conjugated secondary antibody (1:5000). The quantification of Western blot was performed with Image Lab software for ChemiDoc XRS system (Bio-Rad) and the expression levels of protein were analyzed by ImageJ2x 669 22.214.171.124 software.
Primary antibodies for Western blot include anti-NF-κB P65 (RelA) (CST, 8242S; 1:2,000), anti-phospho-NF-κB P65 (Ser536) (pRelA) (CST, 3033S; 1:1,000), anti-β-Actin (Santa Cruz, sc-69879; 1:5000).
Cells seeded on microscope coverslips were fixed with 4% formaldehyde for 20–30 min, permeabilized with 0.4% Triton X-100 in PBS for 10–20 min, and blocked with 10% donkey serum in PBS for 1 h at room temperature. Cells were then incubated with primary antibody (diluted with 1% donkey serum in PBS) overnight at 4 °C and fluorescence-labeled secondary antibody (Invitrogen; 1:500 diluted with 1% donkey serum in PBS) at room temperature for 1 h the next day. Hoechst 33342 (Invitrogen; 1:1,000) was used to stain nuclear DNA.
Primary antibodies for immunofluorescence include anti-NANOG (Abcam, ab21624; 1:100), anti-SOX2 (Santa Cruz, sc-17320; 1:200), anti-OCT4 (Santa Cruz, sc-365509; 1:200), anti-TUJ1 (Sigma, T2200; 1:500), anti-α-SMA (Sigma, A5228; 1:200), anti-FOXA2 (CST, 8186S; 1:200), anti-Vimentin (Abcam, ab8978; 1:250), anti-α-Tubulin (Sigma, T5168; 1:500), anti-Vinculin (Sigma, V9131; 1:100), anti-ZOI (Abcam, ab96587; 1:200), anti-ClaudinV (Abcam, ab15106; 1:200), anti-SM22 (Abcam, ab14106; 1:200), anti-Calponin (Dako, M3556; 1:200), anti-vWF (Dako, A0082; 1:200), anti-eNOS (BD, 610296; 1:100), anti-VE-cadherin (CD144) (CST, 2158S; 1:100), anti-human CD31-FITC (BD biosciences, 557508, 1:100), anti-Ki67 (Vector Laboratories, ZA0731; 1:500), Phalloidin (F-actin) (Invitrogen, A22287; 1:50), anti-NF-κB P65 (RelA) (CST, 8242S; 1:200).
RNA-seq library construction and data quality control
VSMCs and VECs at passage 2 were collected for RNA-seq analysis using Illumina sequencing platform. RNA sequencing libraries were prepared as previously reported (Geng et al., 2018; Wang et al., 2018a). Briefly, RNA integrity was examined by the Bioanalyzer 2100 system (Agilent Technologies). Sequencing libraries were constructed using NEB Next UltraTM RNA Library Prep Kit for Illumina (NEB) and sequenced on Illumina Hiseq X Ten platform. All of the sequencing reads were cleaned to remove any artificial sequences and reads with more than 10% low-quality bases.
RNA-seq data processing
RNA-seq data processing was performed as previously described (Zhang et al., 2015a; Geng et al., 2018; Wang et al., 2018a). Sequencing reads were trimmed and mapped to hg19 human genome using hisat2 software (v2.0.4) (Kim et al., 2015). The transcriptional expression level of each gene was counted by HTSeq (v0.6.1) (Anders et al., 2015). Differentially expressed genes (DEGs) were computed using DESeq2 with the threshold of adjusted P value (Benjamini-Hochberg) less than 0.05 and |Log2(fold change)| more than 1 (Love et al., 2014). The correlation between replicates of each sample was evaluated by the Pearson correlation coefficient (R), which was based on DESeq2 regularized-logarithm (rLog) normalized read count. Gene ontology (GO) and pathway enrichment analysis was conducted by Metascape (http://www.metascape.org/) (Tripathi et al., 2015). Gene set enrichment analysis (GSEA) was performed using GSEA software (Subramanian et al., 2007). Transcription levels of NF-κB target genes were analyzed as below. The NF-κB target genes were identified according to database (Siggers et al., 2015; Li et al., 2017). NF-κB target genes with a P value less than 0.01 were taken into consideration and P values of Log2(Fold change) between NF-κB target genes (P < 0.01) and other genes were calculated by Two-sample Kolmogorov-Smirnov test. The RNA-seq data have been deposited to the NCBI Gene Expression Omnibus (GEO) database with accession number GSE124500.
3D-SIM super-resolution microscopy and image analysis
After cells were stained, 3D-SIM images of VSMCs and VECs were acquired on the DeltaVision OMX V3 imaging system (GE Healthcare) with a 100×/1.40 NA oil objective (Olympus UPlanSApo), solid-state multimode lasers (488 nm, 405 nm, 561 nm) and electron-multiplying CCD (charge-coupled device) cameras (Evolve 512 × 512, Photometrics). Serial Z-stack sectioning was done at 125 nm intervals for SIM mode. To obtain optimal images, immersion oil with refractive indices of 1.516 was used for cells on glass coverslips. The microscope was routinely calibrated with 100 nm fluorescent spheres to calculate both the lateral and axial limits of image resolution. SIM image stacks were reconstructed using softWoRx 6.1.1 (GE Healthcare) with the following settings: pixel size 39.5 nm; channel-specific optical transfer functions; Wiener filter constant 0.0010; discard Negative Intensities background; drift correction with respect to first angle; custom K0 guess angles for camera positions. The reconstructed images were further processed for maximum-intensity projections with softWoRx 6.1.1. Pixel registration was corrected to be less than 1 pixel for all channels using 100 nm Tetraspeck beads.
For imaging and analysis of cytoskeletal structures, the statement of the normal cytoskeletal structures were based on the morphology of the WTs in the representative picture. The normal cytoskeletal structures are as follows: the microfilaments should without obvious robust bundles or nodular structures (Domenga et al., 2004; Tikka et al., 2012); the intermediate filaments and microtubules should be in the form of a filament-like structure distributed in a network without significant aggregation (Fogl et al., 2016; Fuertes-Alvarez et al., 2018; Tu et al., 2018); the adhesion junction protein vinculin should be in a punctiform structure and co-localizes with the microfilaments near the cell membrane (Tikka et al., 2012); the tight junction proteins are membrane-localized proteins that resemble the pattern of other VEC surface markers such as CD31 and CD144 (Lee et al., 2018; Zhang et al., 2018b).
CADASIL was compared with the mean of the two WTs using unpaired t-test. RT-qPCR results were analyzed using one-way ANOVA and Bonferroni Post Hoc test. All results of experiments with TNFα treatment were analyzed by two-way ANOVA and Sidak’s multiple comparisons test. All the analyses were conducted using Graph-Pad Prism Software and P value less than 0.05 were considered statistically significant. P > 0.05 (NS), P < 0.05 (*), P < 0.01 (**) and P < 0.001 (***).
We are grateful to Lei Bai, Ruijun Bai and Shikun Ma for administrative assistance, to Xin Zhang, Wei Li and Xiaoqian Zhang for their technical assistance. We thank to Sai Yang (IBP, CAS), Na Li (IBP, CAS), Shuo Guo (IBP, CAS), Xinyi Wu (IBP, CAS), Mengfei Wang (IBP, CAS) and Shengnan Cui (IBP, CAS) for management of laboratory animals, to Lei Zhou (IBP, CAS) for providing veterinary care. We thank Tongxin Niu at HPC-Service Station in Center for Biological Imaging (IBP, CAS) for the management of bioinformatic analysis station. We are grateful to Junying Jia (IBP, CAS) and Shuang Sun (IBP, CAS) for their help in the FACS experiment. We would like to thank Shuoguo Li (IBP, CAS) for her help in taking and analyzing SIM images. This work was supported by the National Key Research and Development Program of China (2018YFC2000100), the Strategic Priority Research Program of the Chinese Academy of Sciences (XDA16010100), the National Key Research and Development Program of China (2017YFA0103304, 2017YFA0102802, 2018YFA0107203, 2016YFC1300605, 2015CB964800 and 2014CB910503), the National Natural Science Foundation of China (81625009, 81330008, 91749202, 91749123, 31671429, 81671377, 81771515, 31601109, 31601158, 81701388, 81601233, 81471414, 81870228, 81822018, 81801399, 31801010, 81801370, 81861168034 and 81471185), Program of Beijing Municipal Science and Technology Commission (Z151100003915072), Key Research Program of the Chinese Academy of Sciences (KJZDEWTZ-L05), Beijing Municipal Commission of Health and Family Planning (PXM2018_026283_000002), Advanced Innovation Center for Human Brain Protection (117212), and the State Key Laboratory of Membrane Biology. J.C.I.B was supported by UCAM, AFE, Pedro Guillen, Helmsley and Moxie Foundations.
Ac-LDL, acetylated low density lipoprotein; CADASIL, cerebral autosomal dominant arteriopathy with subcortical infarcts and leukoencephalopathy; CAPE, caffeic acid phenethyl ester; ESCs, embryonic stem cells; GO-BP, gene ontology biological processes; GO, gene ontology; GOM, granular osmiophilic material; GSEA, gene set enrichment analysis; iPSCs, induced pluripotent stem cells; NO, nitric oxide; NOD/SCID, non-obese diabetic severe combined immunode ficiency; TNFα, tumor necrosis factor alpha; VECs, vascular endothelial cells; VSMCs, vascular smooth muscle cells; MSCs, mesenchymal stem cells; WT, wildtype.
Compliance with ethics guidelines
The authors declare no conflict of interest. All institutional and national guidelines for the care and use of laboratory animals were followed.
- Craggs LJ, Fenwick R, Oakley AE, Ihara M, Kalaria RN (2015) Immunolocalization of platelet-derived growth factor receptor-beta (PDGFR-beta) and pericytes in cerebral autosomal dominant arteriopathy with subcortical infarcts and leukoencephalopathy (CADASIL). Neuropathol Appl Neurobiol 41:557–570PubMedPubMedCentralCrossRefGoogle Scholar
- Di Donato I, Bianchi S, De Stefano N, Dichgans M, Dotti MT, Duering M, Jouvent E, Korczyn AD, Lesnik-Oberstein SA, Malandrini A et al (2017) Cerebral autosomal dominant arteriopathy with subcortical infarcts and leukoencephalopathy (CADASIL) as a model of small vessel disease: update on clinical, diagnostic, and management aspects. BMC Med 15:41PubMedPubMedCentralCrossRefGoogle Scholar
- Fogl C, Mohammed F, Al-Jassar C, Jeeves M, Knowles TJ, Rodriguez-Zamora P, White SA, Odintsova E, Overduin M, Chidgey M (2016) Mechanism of intermediate filament recognition by plakin repeat domains revealed by envoplakin targeting of vimentin. Nat Commun 7:10827PubMedPubMedCentralCrossRefGoogle Scholar
- Fuertes-Alvarez S, Maeso-Alonso L, Villoch-Fernandez J, Wildung M, Martin-Lopez M, Marshall C, Villena-Cortes AJ, Diez-Prieto I, Pietenpol JA, Tissir F et al (2018) p73 regulates ependymal planar cell polarity by modulating actin and microtubule cytoskeleton. Cell Death Dis 9:1183PubMedPubMedCentralCrossRefGoogle Scholar
- Gatti JR, Zhang X, Korcari E, Lee SJ, Greenstone N, Dean JG, Maripudi S, Wang MM (2018) Redistribution of mature smooth muscle markers in brain arteries in cerebral autosomal dominant arteriopathy with subcortical infarcts and leukoencephalopathy. Transl Stroke Res. https://doi.org/10.1007/s12975-018-0643-x CrossRefPubMedGoogle Scholar
- Joutel A, Monet-Lepretre M, Gosele C, Baron-Menguy C, Hammes A, Schmidt S, Lemaire-Carrette B, Domenga V, Schedl A, Lacombe P et al (2010) Cerebrovascular dysfunction and microcirculation rarefaction precede white matter lesions in a mouse genetic model of cerebral ischemic small vessel disease. J Clin Invest 120:433–445PubMedPubMedCentralCrossRefGoogle Scholar
- Miao Q, Paloneva T, Tuominen S, Poyhonen M, Tuisku S, Viitanen M, Kalimo H (2004) Fibrosis and stenosis of the long penetrating cerebral arteries: the cause of the white matter pathology in cerebral autosomal dominant arteriopathy with subcortical infarcts and leukoencephalopathy. Brain Pathol 14:358–364PubMedCrossRefGoogle Scholar
- Monet-Lepretre M, Haddad I, Baron-Menguy C, Fouillot-Panchal M, Riani M, Domenga-Denier V, Dussaule C, Cognat E, Vinh J, Joutel A (2013) Abnormal recruitment of extracellular matrix proteins by excess Notch3 ECD: a new pathomechanism in CADASIL. Brain 136:1830–1845PubMedPubMedCentralCrossRefGoogle Scholar
- Okeda R, Arima K, Kawai M (2002) Arterial changes in cerebral autosomal dominant arteriopathy with subcortical infarcts and leukoencephalopathy (CADASIL) in relation to pathogenesis of diffuse myelin loss of cerebral white matter: examination of cerebral medullary arteries by reconstruction of serial sections of an autopsy case. Stroke 33:2565–2569PubMedCrossRefGoogle Scholar
- Panahi M, Yousefi Mesri N, Samuelsson E-B, Coupland KG, Forsell C, Graff C, Tikka S, Winblad B, Viitanen M, Karlström H et al (2018) Differences in proliferation rate between CADASIL and control vascular smooth muscle cells are related to increased TGFβ expression. J Cell Mol Med 22:3016–3024PubMedPubMedCentralCrossRefGoogle Scholar
- Sweeney C, Morrow D, Birney YA, Coyle S, Hennessy C, Scheller A, Cummins PM, Walls D, Redmond EM, Cahill PA (2004) Notch 1 and 3 receptor signaling modulates vascular smooth muscle cell growth, apoptosis, and migration via a CBF-1/RBP-Jk dependent pathway. FASEB J 18:1421–1423PubMedCrossRefGoogle Scholar
- Tikka S, Ng YP, Di Maio G, Mykkanen K, Siitonen M, Lepikhova T, Poyhonen M, Viitanen M, Virtanen I, Kalimo H et al (2012) CADASIL mutations and shRNA silencing of NOTCH3 affect actin organization in cultured vascular smooth muscle cells. J Cereb Blood Flow Metab 32:2171–2180PubMedPubMedCentralCrossRefGoogle Scholar
- Ye L, Chang YH, Xiong Q, Zhang P, Zhang L, Somasundaram P, Lepley M, Swingen C, Su L, Wendel JS et al (2014) Cardiac repair in a porcine model of acute myocardial infarction with human induced pluripotent stem cell-derived cardiovascular cells. Cell Stem Cell 15:750–761PubMedPubMedCentralCrossRefGoogle Scholar
Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made.