Patent Application
20230089966
The contents of the electronic sequence listing (960296.04319.xml; Size: 48,340 bytes; and Date of Creation: Sep. 14, 2022) is herein incorporated by reference in its entirety.
Vascular mural cells, which encompass microvessel-associated pericytes and large vessel-associated vascular smooth muscle cells (VSMCs), regulate blood vessel development, stability, and vascular tone. In the brain, mural cells regulate resting cerebral blood flow, neurovascular coupling, blood-brain barrier development and maintenance, and neuron survival. Brain mural cells are also implicated in the pathogenesis of neurological disorders including Alzheimer's disease and cerebral autosomal dominant arteriopathy with subcortical infarcts and leukoencephalopathy (CADASIL).
In contrast to the mesodermal origin of most mural cells, those in the face and forebrain are derived from the neural crest. During embryogenesis, cranial neural crest-derived mesenchyme (mesectoderm) surrounds the anterior neural tube, and mural cells are specified and invade the developing prosencephalon alongside mesoderm-derived endothelial cells from the perineural vascular plexus. This neural crest-derived mesenchyme also forms the meninges, facial bone, cartilage, and connective tissue, and portions of the skull. Molecular signals controlling specification of neural crest-derived mesenchyme to these diverse fates are poorly understood; however, endothelium-derived signals likely direct mural cell differentiation. In vivo loss of function experiments have suggested roles for TGF-β, PDGF, and Notch signaling in this process. Notably, NOTCH3 mutations form the genetic basis of CADASIL, and studies in Zebrafish have implicated Notch signaling in brain pericyte proliferation and specification of pericytes from naïve neural crest-derived mesenchyme. It is difficult, however, to discriminate between deficits in specification/differentiation and recruitment of mural cells to nascent vessels in most in vivo studies. Thus, in vitro models are complementary and can provide mechanistic insight into the effects of molecular factors on neural crest differentiation.
Human pluripotent stem cells (hPSCs) are a promising in vitro model system for such studies, as they can generate naïve, multipotent neural crest cells, potentially account for species differences in mural cell phenotype, and the resulting cells could be employed in diverse in vitro modeling applications. We recently demonstrated that brain pericyte-like cells could be differentiated from hPSC-derived neural crest via treatment with serum-supplemented E6 medium. Other protocols for generating hPSC-derived brain pericyte-like cells via a neural crest intermediate use PDGF-BB and/or FGF2 but each protocol adds these factors to serum-containing media. The sufficiency of serum to cause differentiation of neural crest cells makes interrogation of specific molecular factors difficult, motivating development of a serum-free differentiation scheme. Furthermore, while existing hPSC-derived pericyte-like cells have many molecular and functional attributes of pericytes in vivo, they lack expression of some key brain mural cell genes and have aberrant expression of some fibroblast-associated genes, features also observed in cultured primary brain pericytes. This further motivates development of a new protocol for hPSC differentiation to brain mural cells with an improved molecular phenotype.
Needed in the art is an improved method of creating hPSC-derived mural cells that can be used in models and for drug discovery and testing purposes.
In one aspect, the present disclosure provides a method of producing a population of mural cells comprising the steps of: a) increasing Notch expression and/or signaling in a population of p75-NGFR+HNK-1+ neural crest (NC) cells; and b) culturing the Notch-activated NC cells in serum-free medium for a sufficient time to differentiate the NC cells into NOTCH3+PDGFRβ+RGS5+ brain mural cells.
In another aspect, the present disclosure provides a method of creating a population of NOTCH3+PDGFRβ+RGS5+ brain mural cells comprising: a) culturing hPSCs in E6-CSFD medium for about 15 days to produce p75-NGFR+HNK-1+ NCSCs, b) sorting p75-NGFR+ cells and re-plating the p75-NGFR+ cells of step (a) to produce a population of p75-NGFR+ NCSCs; c) activating notch signaling in the sorted p75-NGFR+HNK-1+ NCSCs of step b), and d) culturing the cells of step (c) in serum free medium for a sufficient time to differentiate NOTCH3+PDGFRβ+RGS5+ brain mural cells.
In another aspect, the disclosure provides a population of NOTCH3+PDGFRβ+RGS5+ brain mural cells produced by the methods described herein.
In a further aspect, the disclosure provides a BBB model, wherein the model comprises the population of NOTCH3+PDGFRβ+RGS5+ brain mural cells described herein and brain microvascular endothelial cells (BMECs), wherein the BBB model is capable of forming tight junctions. The BBB model may be an isogenic BBB model. The BBB model may also include a permeable membrane.
In a still further aspect, methods of using the NOTCH3+PDGFRβ+RGS5+ brain mural cells in in vitro assays are also provided. The cells may be used for drug screening and tissue development or assays.
The patent or application file contains at least one drawing executed in color. Copies of this patent or patent application publication with color drawing(s) will be provided by the Office upon request and payment of the necessary fee.
The present invention is based in part on the surprising finding that activation of Notch3 or Notch1 signaling directed the differentiation of hPSC-derived neural crest to brain mural cells. Further, overexpression of Tbx2 (SEQ ID NO:5 and 6), another mural cell-enriched transcription factor similar to Notch3 and Notch1, did not similarly induce brain mural cells. Because ligand-induced activation of Notch signaling requires complex cell-cell interactions and ligand endocytosis, the inventors activated Notch signaling by lentiviral overexpression of the human Notch3 or Notch1 intracellular domain in neural crest cells maintained in serum-free medium. The resulting cells were PDGFRβ+ and displayed robust upregulation of the mural cell genes HEYL, RGS5, TBX2, and FOXS1. Supplementation of additional molecular factors did not substantially improve the transcriptional profile of the resulting cells. Thus, Notch3 or Notch1 signaling is sufficient to direct differentiation of neural crest to brain mural cells under serum-free conditions, and thus establishes a new, serum-free protocol for generation of brain mural cells from hPSCs. These in vitro derived brain mural cells can be used in CNS drug screening, BBB models and development studies and disease modeling applications.
Abbreviations used in the present disclosure include, blood-brain barrier, BBB; brain microvascular endothelial cells, BMECs; central nervous system, CNS; E6 medium supplemented with CHIR99021, SB431542, FGF2, and dorsomorphin, E6-CSFD; endothelial cells, ECs; endothelial growth factor medium 2, EGM-2; green fluorescent protein, GFP; human embryonic stem cells, hESCs; human pluripotent stem cells, hPSCs; human umbilical vein endothelial cells, HUVECs; induced pluripotent stem cells, iPSCs; Notch1 intracellular domain, N1ICD; Notch3 intracellular domain, N3ICD; neural crest stem cells, NCSC; neurovascular unit, NVU; vascular smooth muscle cells, VSMCs.
Brain pericytes and vascular smooth muscle cells (VSMCs), collectively termed mural cells, regulate development and function of the blood-brain barrier (BBB) and control brain blood flow. Unlike the mesoderm-derived mural cells of other organs, forebrain mural cells (also called brain mural cells or vascular mural cells) are derived from the neural crest. Molecular signals controlling mural cell differentiation are poorly understood, with loss of function experiments suggesting roles for TGF-β, PDGF, and Notch signaling. Existing in vitro models of human brain mural cells derived both from primary cultures and human pluripotent stem cells (hPSCs) have markedly reduced expression of key mural cell genes, including NOTCH3, compared to in vivo samples, and require serum-supplemented culture media. The present invention fulfills a need for in vitro derived mural cells that have key aspects of the mural cells and proper gene expression that can be used in vitro for creating BBB models and development and drug discovery applications.
The present invention provides populations of in vitro derived brain mural cells and methods of producing brain mural cells under serum free conditions, allowing for their use in studies allowing for standardization of conditions and reproducibility of the components in the culture media, which is ideal for analysis. These brain mural cells can be used for in vitro BBB models, 3D models of blood brain barrier and other tissue and chip technology that can be used to study blood brain barrier properties, development and therapeutics. As demonstrated in the Examples, the overexpression of the human Notch3 intracellular domain (N3ICD) or human Notch1 (N1ICD) in neural crest cells directed mural cell differentiation under serum free conditions. Unexpectedly, while other factors are thought to play a role (e.g., TGFβ, TBX2), these factors did not result in the differentiation of mural cells from neural crest stem cells as described in the Examples. Thus, the present invention provides a novel serum-free method of in vitro deriving brain mural cells for study and down-stream applications.
The in vitro derived brain mural cells of the present invention are NOTCH3+PDGFRβ+RGS5+ brain mural cells. These mural cells of the present invention can form both smooth muscle cells, which line arterioles and venules, and pericytes, which are associated with smaller microvessels and capillaries. Preferably, the methods produce a cell population that is at least 90% NOTCH3+PDGFRβ+RGS5+ brain mural cells, preferably at least 95% NOTCH3+PDGFRβ+RGS5+ brain mural cells. The NOTCH3+PDGFRβ+RGS5+ brain mural cells may also express one or more additional marker associated with mural cells, e.g., FOXS1, TBX2, and HEYL. Additionally, the mural cells express pericyte-specific markers (e.g., KCNJ8) at certain timepoints, but additional factors may need to be used for maintenance of this phenotype or further differentiation.
In one aspect, the present disclosure provides a method of producing a population of mural cells. The method comprises (a) increasing Notch expression and/or activation in a population of p75-NGFR+HNK-1+ neural crest (NC) cells; and (b) culturing the Notch-activated NC cells in serum-free medium for a sufficient time to differentiate the NC cells into NOTCH3+PDGFRβ+RGS5+ brain mural cells. Suitably, in some embodiments, the culturing step of Notch-activated NC cells in serum free medium to obtain NOTCH3+PDGFRβ+RGS5+ brain mural cells is at least 6 days. The brain mural cells may be cultured and split for additional passages for up to 60 days.
It is contemplated that a number of different methods and strategies may be used for increasing the Notch expression and/or signaling within the NC cells to promote differentiation into mural cells. For example, Notch expression or Notch signaling within the NC cell may be accomplished by methods known in the art to activate the Notch signaling pathway. Some examples, include, for example, (i) introducing a exogenous construct encoding at least an intracellular domain of Notch receptor and capable of expressing at least the intracellular domain within the NC cell, although additional Notch receptor and/or ligand sequences may also be included; (ii) culturing the NC cells in serum free medium in the presence of Notch ligands (e.g., DLL4, JAG2, etc.); (iii) co-culturing the NC cells with cells overexpressing Notch ligands (e.g., feeder cell line, etc.) or (iv) activating Notch pathway using a Notch activation factor. Suitable methods of activating the Notch pathway are known and understood in the art. In one aspect, an exogenous construct comprises a Notch receptor, Notch ligand, or a Notch activating factor or active fragments thereof. In one example, the Notch receptor comprises at least a Notch intracellular domain (e.g., Notch 3 or Notch 1 intracellular domain) and capable of expressing the Notch intracellular domain.
In some embodiments, the construct encoding a Notch receptor, Notch ligand, or fragment thereof or Notch activating factor may suitably be a vector. In a preferred embodiment, the construct may be a viral vector, for example, a lentiviral vector that allows for integration and stable expression of the Notch intracellular domain encoded within the cell. In other embodiments, expression vectors may be used that allow for transient expression of the Notch intracellular domain within the cell. In other aspects, other methods may be used to overexpress Notch within the NC cells, for example, either the NC cells or the hPSCs used to derive the NC can be genetically modified with a construct (e.g. by viral, transposon, CRISPR-based strategies) that has a inducible construct for notch intracellular domain expression (e.g., doxycycline-inducible). Suitable doxycycline vectors and constructs are known in the art, and expression is then inducible by the addition of doxycycline or other suitable inductor into the culture medium.
In some embodiments the vector may comprise a polynucleotide encoding the intracellular domain of Notch3, for example, SEQ ID NO:1 or another polynucleotide capable of encoding SEQ ID NO: 2. Alternatively, the vector may comprise a polynucleotide encoding the intracellular domain of Notch1, for example SEQ ID NO: 3 or another polynucleotide capable of encoding SEQ ID NO: 4. Due to the degeneracy of the genetic code those of skill in the art will appreciate that the polypeptides of SEQ ID NO: 2 and 4 may be encoded for by many distinct polynucleotides. In addition, the polypeptides can also maintain function with a small number of amino acid changes. Thus also encompassed herein are polynucleotides and polypeptides having at least 90%, 92%, 94%, 95%, 97% 98% or 99% identity to the sequences provided in SEQ ID NO: 1-4. The vector may comprise additional sequences, including promoter sequences. Heterologous promoters useful in the practice of the present invention include, but are not limited to, constitutive, inducible, temporally-regulated, developmentally regulated, chemically regulated, tissue-preferred, tissue-specific promoters and cell-type specific. The heterologous promoter may be a plant, animal, bacterial, fungal, or synthetic promoter. Suitable promoters are known and described in the art. Promoters may include the EF-1alpha, SV40, CMV, UBC, PGK or CAGG. The vector may additionally comprise one or more IRES element, enhancer element, translation initiation sequence, ribosomal binding site, start codon, termination codon, transcriptional termination sequence, targeting sequence and/or tag.
In another aspect, the NC cells may be cultured in the presence of excess Notch ligands. Suitable means of culturing cells with notch ligands include, for example, culturing the NC cells in the presence of beads coated with Notch ligands (e.g. DLL4 or JAG2). Other suitable notch ligands may also be used (e.g., DSL ligands, Delta and Serrate, three of which belong to the Delta-like family (DLL1, DLL3 and DLL4) and two belong to the Jagged family of Serrate homologs, Jagged 1 and 2 (also known as JAG1 and JAG2, respectively) and their use can be determined by one skilled in the art). Suitable beads are known in the art and comprise, for example, agarose, polymer or magnetic beads. Suitable methods of deriving beads coated with notch ligands are known in the art, for example, surfaces of microbeads are coated with Streptavidin which then binds the biotin attached to the anti-HIS antibody in which recombinant DLL4 with a HIS tag can be attached to the antibody. This method allows for the DLL4 to be immobilized and presented in a highly directional manner on the surface of the beads. Alternatively, for example, recombinant DLL4-Fc or JAG2-Fc fusion proteins can be attached to agarose beads coated with Protein A or Protein G, in which the Fc domain binds to Protein A or Protein G.
In another aspect, the NC cells may be cultured on culture plates coated with Notch ligands (e.g., DLL4 or JAG2). In some embodiments, the plates may be coated with collagen or Matrigel prior to incubation with Notch ligand. Methods of coating plates with proteins including notch are readily understood and known in the art.
In another aspect, the NC cells can be co-cultured with a second cell type that has been genetically altered to overexpress Notch ligands. Suitable co-culture cells are readily known and available in the art.
As used herein, the term “construct”, “nucleic acid construct” or “DNA construct” refers to an artificially constructed (i.e., not naturally occurring) DNA molecule that is capable of expressing the polypeptide. Nucleic acid constructs may be part of a vector that is used, for example, to transform a cell. The term “vector” refers to a nucleic acid molecule capable of propagating another nucleic acid to which it is linked. The term includes the vector as a self-replicating nucleic acid structure as well as the vector incorporated into the genome of a host cell into which it has been introduced. Certain vectors are capable of directing the expression of nucleic acids to which they are operatively linked. Such vectors are referred to herein as “expression vectors”. Vectors suitable for use with the present invention comprise the constructs described herein and heterogeneous sequence necessary for proper propagation of the vector and expression of the encoded polypeptide. Preferably, the constructs are packaged in a vector suitable for delivery into a mammalian cell including but not limited to, an adeno-associated viral (AAV) vector, a lentiviral vector, or a vector suitable for transient transfection. As used herein, the term “vector,” “virus vector,” “delivery vector” (and similar terms) generally refers to a virus particle that functions as a nucleic acid delivery vehicle, and which comprises the viral nucleic acid (i.e., the vector genome) packaged within the virion. Suitable vectors are known and commercially available in the art. A skilled artisan will be familiar with the elements and configurations necessary for vector construction to encode the constructs described herein.
The term “neural crest (NC) cells” or “neural crest stem cells (NCSC)” are used herein interchangeably to refer to a multipotent stem cell or progenitor population capable of forming peripheral neurons and mesenchymal derivatives including adipocytes, osteocytes, and chondrocytes, among other cell types. NCSCs are the embryonic precursor to forebrain pericytes. As described in the Examples, the neural crest cells used in the methods described herein are differentiated from human pluripotent stem cells, including induced pluripotent stem cells. Suitable methods of deriving neural crest cells are described in US Patent Publication No. US2020/0017827 and Stebbins et al., 2019, both of which are incorporated by reference in their entirety. Neural crest cells are identified by expression of key neural crest markers, including, for example, at least p75-NGFR and HNK-1 (B3GAT1), and can express one or more additional neural crest markers. Cells can be sorted during differentiation as p75-NGFR+ to obtain a homogenous population of p75-NGFR+ neural crest stem cells (NCSC). Such NCSCs can be expanded in culture before use as the starting population for deriving the mural cells of the present invention. The neural crest cells can be denoted as p75-NGFR+HNK-1+ neural crest (NC) cells, and the starting population of p75-NGFR+HNK-1+ NC cells can be at least 90% pure, alternatively at least 95% pure, alternatively at least 98% p75-NGFR+HNK-1+ NC cells.
The present methods provide advantages of deriving mural cells from those in the art in that the mural cells are derived from NCSCs in serum free medium wherein the medium is defined. The term “defined culture medium” is used herein to indicate that the identity and quantity of each medium ingredient is known. As used herein, the terms “chemically-defined culture conditions,” “fully defined, growth factor free culture conditions,” and “fully-defined conditions” indicate that the identity and quantity of each medium ingredient is known and the identity and quantity of supportive surface is known. As used herein the term “xenogen-free” refers to medium that does not contain any products obtained from a non-human animal source. As used herein, the term “serum albumin-free” indicates that the culture medium used contains no added serum albumin in any form, including without limitation bovine serum albumin (BSA) or any form of recombinant albumin. Standardizing culture conditions by using a chemically defined culture medium minimizes the potential for lot-to-lot or batch-to-batch variations in materials to which the cells are exposed during cell culture. Accordingly, the effects of various differentiation factors are more predictable when added to cells and tissues cultured under chemically defined conditions. As used herein, the term “serum-free” refers to cell culture materials that do not contain serum or serum replacement, or that contain essentially no serum or serum replacement. For example, an essentially serum-free medium can contain less than about 1%, 0.9%, 0.8%, 0.7%, 0.6%, 0.5%, 0.4%, 0.3%, 0.2%, or 0.1% serum. “Serum free” also refers to culture components free of serum obtained from animal blood and of animal-derived materials, which reduces or eliminates the potential for cross-species viral or prion transmission. Further, serum-containing medium is not chemically defined, producing a degree of variability in the culture conditions. Suitable defined media include, but are not limited to, E8 medium and E6 medium.
Any appropriate method can be used to detect expression of biological markers characteristic of cell types described herein. For example, the presence or absence of one or more biological markers can be detected using, for example, RNA sequencing, immunohistochemistry, polymerase chain reaction, qRT-PCR, or other technique that detects or measures gene expression. Suitable methods for evaluating the above-markers are well known in the art and include, e.g., qRT-PCR, RNA-sequencing, and the like for evaluating gene expression at the RNA level. Quantitative methods for evaluating expression of markers at the protein level in cell populations are also known in the art. For example, flow cytometry is typically used to determine the fraction of cells in a given cell population that express (or do not express) a protein marker of interest (e.g., NOTCH3, GFP, PDGFRβ). In some cases, cell populations obtained by the differentiation methods of this disclosure comprise at least 80%, 85%, 90%, 95% and preferably at least 98% NOTCH3+PDGFRβ+RGS5+ brain mural cells.
As discussed above, in some embodiments, the p75-NGFR+HNK-1+ neural crest (NC) cells are derived from pluripotent stem cells, for example, induced pluripotent stem cells. In one embodiment, the method further comprises culturing human pluripotent cells in E6-CSFD medium for about 15 days to produced p75-NGFR+HNK-1+ NCSCs. NCSCs maintained in E6-CSFD retained neural crest marker expression and did not develop expression of pericyte or mural cell markers.
In general, the method comprises the steps described below in the Examples. Typically, the method begins with culturing or maintaining hPSCs in E8 medium. In some embodiments, this culture step is on coated plates, for example, Matrigel™ coated plates. The Examples below disclose a preferred method of singularizing the cells using Accutase and preferred seeding densities. As used herein, the terms “E8 culture medium” and “E8” are used interchangeably and refer to a chemically defined culture medium comprising or consisting essentially of DF3S supplemented by the addition of insulin (20 μg/mL), transferrin (10.67 ng/mL), human FGF2 (100 ng/mL), and human TGFβ1 (Transforming Growth Factor Beta 1) (1.75 ng/mL). The medium can be prepared based on the formula in previous publication (Chen et al., (2011) Nature Methods. 8(4), 424-429). As an alternative, the medium is also available from ThermoFisher/Life Technologies Inc. as Essential 8, or from Stem Cell Technologies as TeSR-E8.
Further differentiation steps include using E6 medium that is described herein and in U.S. Patent Publication No. 2014/0134732. Preferably, the chemically defined medium comprises DMEM/F-12. E6 medium contains DMEM/F12; L-ascorbic acid-2-phosphate magnesium (64 mg/1); sodium selenium (14 μg/1); insulin (20 mg/1); NaHCO3 (543 mg/1); and transferrin (10.7 mg/1). E6-CSFD is E6 medium supplemented with CHIR99021, SB431542, FGF2, dorsomorphin, and heparin. Suitable ranges of the factors for inclusion in E6 medium to produce E6-CSFD media includes, for example, about 0.5-5 μM CHIR99021 (preferably 1 μM), a GSK3I3 inhibitor to promote WNT signaling; 5-20 μM SB431543 (preferably 10 μM), an ALK5 antagonist to inhibit Activin/Nodal/TGFβ signaling; 5-100 ng/ml FGF2 (preferably 10 ng/mL); about 0.5-2 μM dorsomorphin (preferable 1 μM), a BMP type I receptor inhibitor; and about 2-200 μg/ml heparin (preferably 22.5 μg/ml). One exemplary formulation of E6-CSFD is 1 μM CHIR99021; 10 μM SB431543; 10 ng/mL FGF2 (E6-CSF); and 1 μM CHIR99021, 1 μM dorsomorphin, and 22.5 μg/ml heparin.
One would then culture the in vitro hPSCs described above in E6-CSFD medium for about 15 days to produce a population comprising NCSCs. Suitable, the cells can be cultured for at least 15 days, and can be maintained in culture to about 60 days. One would then typically sort and re-plate the NCSC cells, which express HNK-1 and p75-NGFR (e.g., p75-NGFR+HNK-1+ NCSCs).
In one embodiment, the method further comprises differentiating the p75-NGFR+HNK-1+NSCs from human pluripotent stem cells. The method comprises culturing hPSC in E6-CSFD medium for about 15 days to produced p75-NGFR+HNK-1+ NCSC cells, subsequently sorting p75-NGFR+ cells from the population and re-plating the p75-NGFR+ cells of step to produce a population of p75-NGFR+ NCSCs. Methods of sorting the p75-NGFR+ cells are known to one skilled in the art and include, but are not limited to, fluorescence activated cell sorting (FACS) and magnetic-activated cell sorting (MACS), among others. A preferred method of sorting the cells is MACS.
The population of cells produced from hPSCs is a p75-NGFR+HNK-1+AP-2+ NCSCs which are able to be maintained in culture, e.g., the cells are able to double at least 5 times in culture and still maintain expression p75-NGFR+, HNK-1+, and AP-2+ within the cells. These NCSCs are able to be maintained in culture for at least five passages and maintain p75-NGFR+HNK-1+AP-2+ marker expression and do not express pericyte or mural cell markers (e.g., NG2−, PDGFRβ−, etc). These NCSCs produced by the method described herein are able to maintain the potential to differentiate into neurons and mesenchymal cells, as demonstrated in the Examples below.
The p75-NGFR+HNK-1+ NCSCs may be further cultured and passaged for at least 60 days. The Examples below describe suitable hPSC lines. The human pluripotent stem cells may be embryonic stem cells or induced pluripotent stem cells (iPSCs). The present invention is also meant to employ iPSC lines developed from individual patients or disease models.
As used herein, “pluripotent stem cells” appropriate for use according to a method of the invention are cells having the capacity to differentiate into cells of all three germ layers. Suitable pluripotent cells for use herein include human embryonic stem cells (hESCs) and human induced pluripotent stem cells (iPSCs). As used herein, “embryonic stem cells” or “ESCs” mean a pluripotent cell or population of pluripotent cells derived from an inner cell mass of a blastocyst. See Thomson et al., Science 282:1145-1147 (1998). These cells express Oct-4, SSEA-3, SSEA-4, TRA-1-60 and TRA-1-81 and appear as compact colonies having a high nucleus to cytoplasm ratio and prominent nucleolus. ESCs are commercially available from sources such as WiCell Research Institute (Madison, Wis.). As used herein, “induced pluripotent stem cells” or “iPSCs” mean a pluripotent cell or population of pluripotent cells that may vary with respect to their differentiated somatic cell of origin, that may vary with respect to a specific set of potency-determining factors and that may vary with respect to culture conditions used to isolate them, but nonetheless are substantially genetically identical to their respective differentiated somatic cell of origin and display characteristics similar to higher potency cells, such as ESCs. See, e.g., Yu et al., Science 318:1917-1920 (2007), incorporated by reference in its entirety. Induced pluripotent stem cells exhibit morphological properties (e.g., round shape, large nucleoli and scant cytoplasm) and growth properties (e.g., doubling time of about seventeen to eighteen hours) akin to ESCs. In addition, iPSCs express pluripotent cell-specific markers (e.g., Oct-4, SSEA-3, SSEA-4, Tra-1-60 or Tra-1-81, but not SSEA-1). Induced pluripotent stem cells, however, are not immediately derived from embryos. As used herein, “not immediately derived from embryos” means that the starting cell type for producing iPSCs is a non-pluripotent cell, such as a multipotent cell or terminally differentiated cell, such as somatic cells obtained from a post-natal individual.
In one embodiment, the disclosure provides a method of creating a population of NOTCH3+PDGFRβ+RGS5+ brain mural cells comprising: a) culturing hPSCs in E6-CSFD medium for about 15 days to produce p75-NGFR+HNK-1+ NCSCs, b) sorting p75-NGFR+ cells and re-plating the p75-NGFR+ cells of step (a) to produce a population of p75-NGFR+ NCSCs; c) activating Notch signaling in the sorted p75-NGFR+HNK-1+ NCSCs of step (b), and d) culturing the Notch-activated NC cells in serum free medium for a sufficient time to differentiate NOTCH3+PDGFRβ+RGS5+ brain mural cells. A sufficient amount of time is about six days, and optionally between two and ten days
The present invention also provides an in vitro derived population of NOTCH3+PDGFRβ+RGS5+ brain mural cells. The NOTCH3+PDGFRβ+RGS5+ brain mural cells may be derived from any of the methods described herein. The mural cells may be capable of doubling at least 5 times in culture. The population of cells produced may also express one or more additional mural cell markers, for example, TBX2, endogenous Notch3, FOXS1 and HEYL. In some aspects, the NOTCH3+PDGFRβ+RGS5+ brain mural cells population also may be capable of differentiating further into brain pericytes and vascular smooth muscle cells. Such cells may express additional mural and/or pericyte gene markers including by way of example and not limitation HEYL, HES4, TBX2, FOXS1, FOXF2, and FOXC1, PDGFRB, RGS5, NDUFA4L2, KCNJ8, ABCC9, HIGD1B, IGFBP7, PLXDC1, CSPG4, ADAMTS1, FOXD1, GJA4, PTGIR, and MCAM (CD146).
In some aspects, the NOTCH3+PDGFRβ+RGS5+ brain mural cells population also may be capable of forming functional KATP channels and expressing subunits of the KATP channel including, but not limited to KCNJ8 and ABCC9.
In some aspects, the NOTCH3+PDGFRβ+RGS5+ brain mural cells population also may be capable of forming producing extracellular matrix and expressing extracellular matrix genes, including, but not limited to FN1, COL4A1, COL4A2, COL1A1, and LAMA4.
In some aspects, the NOTCH3+PDGFRβ+RGS5+ brain mural cells population also may express human species-specific genes, including but not limited to SLC6A12; and lack expression of mouse species-specific genes, including but not limited to VTN.
The present disclosure also provides a blood brain barrier model comprising the population of NOTCH3+PDGFRβ+RGS5+ brain mural cells, a permeable membrane and brain microvascular endothelial cells (BMECs) (derived from hPSCs, or primary cultures or cell lines), wherein the BBB model is capable of forming tight junctions.
The NOTCH3+PDGFRβ+RGS5+ brain mural cells can be used for making in vitro models of the BBB. For example, co-culture of BMECs with brain mural cells may improve the BMEC phenotype in co-culture systems, stabilize endothelial cell cord formation in vitro, and induce BMEC properties in primary and hematopoietic stem cell-derived endothelial cells. Thus, the mural cells described herein can be used for producing hPSC-derived BBB models. These BBB models offer the capability for screening of CNS-penetrant therapeutics and can be used to investigate BBB contributions to human disease using patient-derived induced pluripotent stem cells (iPSCs) to derive the cells. Further, for patient-specific modeling of the healthy and diseased BBB, it is paramount to generate mural cells from human iPSCs. The brain mural cells may be used to induce blood-brain barrier (BBB) properties in BMECs in a BBB model, including barrier enhancement and reduction of transcytosis. Incorporating these mural cells with iPSC-derived BMECs, astrocytes, and neurons, one can form an isogenic human NVU model useful for the study of the BBB in CNS health, disease, and therapy.
Use of the mural cells derived herein can be used in blood brain barrier models, for example, those that are described in the art, including, for example, U.S. Ser. No. 13/793,466 (Publication US2017/025935), Ser. No. 13/218,123 (U.S. Pat. No. 8,293,495) and Ser. No. 16/092,450 (Publication US2019/0093084) are drawn to related technology and should be incorporated by reference herein. U.S. Ser. No. 13/218,123 discloses a preferred method of creating an isogenic BBB model (i.e., all of the cell types present are derived for a single patient iPSC line), which comprises BMECs, neurons, and astrocytes, with the use of pericytes in the methods described being able to result in functional improvements to the models. U.S. Ser. No. 13/793,466 discloses an improved BBB model that incorporates retinoic acid (RA). Both of these disclosures provide context for the use of the mural cells of the present invention. Brain mural cells can thus be used to enhance BBB phenotypes in BMECs in these modeling systems.
Mural cells may be co-cultured in a Transwell system (e.g., polystyrene transwell filters with a 0.4 μm pore size) with iPSC-derived BMECs in endothelial cell (EC) medium without FGF2. The transwell coculture system has an upper compartment separated by a Transwell insert containing a microporous semi-permeable membrane that separates the cells in the upper compartment (e.g., CD31+ iPSC-derived BMECs) from the cells in the lower compartment (e.g., the mural cells of the present invention). Suitable EC medium are known in the art and commercially available (e.g., available from Promocell, R&D Systems, Sigma-Aldrich, ScienCell Research Laboratories, Lonza, among others).
Alternatively, mural cells may be co-cultured in direct contact with other cell types, including, for example, endothelial cells, BMECs, astrocytes, and/or neurons. The resulting co-culture models may take the form of cords, networks, aggregates, or “spheroids”. For example, mural cells may be co-cultured with HUVECs to form self-organized aggregates.
All references, patents and patent applications disclosed herein are incorporated by reference with respect to the subject matter for which each is cited, which in some cases may encompass the entirety of the document.
It should be apparent to those skilled in the art that many additional modifications beside those already described are possible without departing from the inventive concepts. In interpreting this disclosure, all terms should be interpreted in the broadest possible manner consistent with the context. Variations of the term “comprising” should be interpreted as referring to elements, components, or steps in a non-exclusive manner, so the referenced elements, components, or steps may be combined with other elements, components, or steps that are not expressly referenced. Embodiments referenced as “comprising” certain elements are also contemplated as “consisting essentially of” and “consisting of” those elements. The term “consisting essentially of” and “consisting of” should be interpreted in line with the MPEP and relevant Federal Circuit's interpretation. The transitional phrase “consisting essentially of” limits the scope of a claim to the specified materials or steps “and those that do not materially affect the basic and novel characteristic(s)” of the claimed invention. “Consisting of” is a closed term that excludes any element, step or ingredient not specified in the claim.
The indefinite articles “a” and “an,” as used herein in the specification and in the claims, unless clearly indicated to the contrary, should be understood to mean “at least one.”
The phrase “and/or,” as used herein in the specification and in the claims, should be understood to mean “either or both” of the elements so conjoined, i.e., elements that are conjunctively present in some cases and disjunctively present in other cases. Multiple elements listed with “and/or” should be construed in the same fashion, i.e., “one or more” of the elements so conjoined. Other elements may optionally be present other than the elements specifically identified by the “and/or” clause, whether related or unrelated to those elements specifically identified. Thus, as a non-limiting example, a reference to “A and/or B”, when used in conjunction with open-ended language such as “comprising” can refer, in one embodiment, to A only (optionally including elements other than B); in another embodiment, to B only (optionally including elements other than A); in yet another embodiment, to both A and B (optionally including other elements); etc.
As used herein in the specification and in the claims, “or” should be understood to have the same meaning as “and/or” as defined above. For example, when separating items in a list, “or” or “and/or” shall be interpreted as being inclusive, i.e., the inclusion of at least one, but also including more than one of a number or list of elements, and, optionally, additional unlisted items. Only terms clearly indicated to the contrary, such as “only one of” or “exactly one of,” or, when used in the claims, “consisting of,” will refer to the inclusion of exactly one element of a number or list of elements. In general, the term “or” as used herein shall only be interpreted as indicating exclusive alternatives (i.e. “one or the other but not both”) when preceded by terms of exclusivity, such as “either,” “one of,” “only one of,” or “exactly one of” “Consisting essentially of,” when used in the claims, shall have its ordinary meaning as used in the field of patent law.
The term “about” or “approximately” means within an acceptable error range for the particular value as determined by one of ordinary skill in the art, which will depend in part on how the value is measured or determined, i.e., the limitations of the measurement system. For example, “about” can mean within 1 or more than 1 standard deviations, per practice in the art. Alternatively, “about” with respect to the compositions can mean plus or minus a range of up to 20%, preferably up to 10%, more preferably up to 5%.
The present invention has been described in terms of one or more preferred embodiments, and it should be appreciated that many equivalents, alternatives, variations, and modifications, aside from those expressly stated, are possible and within the scope of the invention.
Notch3 Directs Differentiation of Brain Mural Cells from Human Pluripotent Stem Cell-Derived Neural Crest
Brain pericytes and vascular smooth muscle cells, collectively termed mural cells, regulate development and function of the blood-brain barrier (BBB) and control brain blood flow. Unlike the mesoderm-derived mural cells of other organs, forebrain mural cells are derived from the neural crest. Molecular signals controlling this differentiation process are poorly understood, with loss of function experiments suggesting roles for TGF-β, PDGF, and Notch signaling. Furthermore, existing in vitro models of human brain mural cells derived both from primary cultures and human pluripotent stem cells (hPSCs) have markedly reduced expression of key mural cell genes, including NOTCH3, compared to in vivo samples, and require serum-supplemented culture media. Thus, we sought to determine whether activation of Notch3 or Notch1 in hPSC-derived neural crest could direct the differentiation of brain mural cells with an improved transcriptional profile.
We generated a bicistronic lentiviral vector encoding the human Notch3 and Notch1 intracellular domain and green fluorescent protein (N3ICD-GFP and N1ICD-GFP respectively). We transduced p75-NGFR+HNK-1+ neural crest cells derived from hPSCs with N3ICD-GFP lentivirus or GFP-only lentivirus in serum-free E6 medium. Compared to GFP-transduced neural crest, N3ICD-GFP-transduced cells exhibited upregulated expression of the mural cell transcripts PDGFRB, RGS5, FOXS1, TBX2, and HEYL. Similar results were obtained with N1ICD-GFP. In contrast, transduction of TBX2-GFP did not produce such an effect. In N3ICD-GFP-transduced cells, we observed increased protein-level expression of PDGFRβ and both full-length and cleaved Notch3. We additionally evaluated the ability of the resulting cells to self-assemble with endothelial cells (ECs) in a cord-formation assay and to induce BBB properties in ECs.
In this Example, the inventors found that expression levels of NOTCH3 and canonical transcriptional targets of Notch signaling were very low in existing hPSC-derived brain pericyte-like cells compared to human brain pericytes in vivo. The inventors found that activation of Notch3 signaling directed the differentiation of hPSC-derived neural crest to brain mural cells under serum-free conditions. Because ligand-induced activation of Notch signaling requires complex cell-cell interactions and ligand endocytosis, the inventors activated Notch signaling by lentiviral overexpression of the human Notch3 intracellular domain in neural crest cells maintained in serum-free medium. The resulting cells were PDGFRβ+ and displayed robust upregulation of the mural cell genes HEYL, RGS5, TBX2, and FOXS1. Supplementation of additional molecular factors did not substantially improve the transcriptional profile of the resulting cells. Thus, this work suggests that Notch3 signaling is sufficient to direct differentiation of neural crest to brain mural cells, and establishes a new, serum-free protocol for generation of brain mural cells from hPSCs.
This data suggests that activation of Notch3 signaling is sufficient to direct differentiation of neural crest to brain mural cells, and that multiple brain mural cell-associated transcription factors are downstream of Notch3 signaling. Established herein is a new, serum-free differentiation protocol for generation of hPSC-derived brain mural cells for downstream in vitro modeling applications.
Transcriptome Analysis of hPSC-Derived Brain Pericyte-Like Cells
We analyzed RNA-sequencing (RNA-seq) gene expression profiles of brain pericyte-like cells differentiated from hPSCs from three independent studies (38, 40, 41). While methodologies differ slightly, all three protocols proceed through a neural crest intermediate and yield cells with molecular and functional characteristics similar to mural cells. We compared these cells to human brain pericytes in vivo, using single cell RNA-seq data from a previous meta-analysis (36). There was moderate correlation between the transcriptome of hPSC-derived pericyte-like cells and in vivo pericytes, and similar expression of some canonical markers such as PDGFRB, ANPEP, CSPG4, COL4A1, IGFBP7, and MYL9 (
Given low expression of NOTCH3 and Notch target genes (e.g., HEYL, HEY2, HES4) in existing hPSC-derived pericyte-like cells and the known roles of Notch signaling in mural cell development (29), we asked whether overexpression of the human Notch3 intracellular domain (N3ICD) in neural crest cells could direct mural cell differentiation. We also evaluated overexpression of Tbx2, a mural cell-enriched transcription factor with similarly low expression in existing hPSC models. We cloned the portion of the NOTCH3 coding sequence (CDS) corresponding to the intracellular domain, and the TBX2 CDS, into bicistronic lentiviral vectors for GFP coexpression (see Methods) (
6 days after lentiviral transduction, N3ICD-GFP-transduced cells had significantly elevated expression of HEYL and endogenous NOTCH3 (using primers targeting the 3′ untranslated region, which is not present in transgene-derived transcripts) compared to GFP controls (
We validated protein-level overexpression of N3ICD via Western blotting with a Notch3 antibody detecting a C-terminal (intracellular domain) epitope. As expected, we observed a significant increase in the intensity of a low molecular weight band corresponding to the Notch transmembrane fragment and intracellular domain in N3ICD-GFP-transduced cultures compared to GFP-transduced cultures (
We used FACS to isolate GFP+ and GFP− cells from cultures 6 days after N3ICD-GFP lentiviral transduction (
We used RNA-seq to obtain transcriptomic profiles of neural crest cells and FACS-isolated GFP− and GFP+ cells from N3ICD-GFP-transduced cultures from four hPSC lines (
The canonical neural crest marker NGFR was downregulated in GFP+ cells compared to both neural crest and GFP− cells, as was LIN28A, which plays a role in neural crest multipotency (49). PDGFRA, which is enriched in fibroblasts compared to mural cells in vivo (45, 50), was nearly absent in GFP+ cells, but expressed by GFP− cells (
We next identified gene sets enriched in GFP+ cells compared to neural crest, using the KEGG and gene ontology-biological process (GO-BP) databases (
Production of vascular basement membrane is a key function of mural cells. We visually observed an apparent enrichment in the amount of ECM produced by cultures transduced with N3ICD-GFP compared to GFP, which we confirmed by decellularization followed by quantification of remaining total protein (see Methods). Compared to GFP-transduced cultures, N3ICD-overexpressing cultures generated approximately 20 times more extracellular matrix per cell despite a slight reduction in total cell number (
Mural cells regulate vascular tone, and while the relative contributions of different mural cell subtypes to neurovascular coupling remain the subject of debate, virtually all mural cells appear capable of contraction, at least under artificial stimuli (55). Potassium (at concentrations causing depolarization) is widely used to assess contractility of pericytes and smooth muscle cells in vitro and in vivo (40, 56). We first used calcium imaging of a N3ICD-GFP-transduced culture to confirm that application of 40 mM KCl led to depolarization and calcium influx (
In the canonical model of Notch signaling, Notch intracellular domains (NICDs) activate transcription of a small number of transcription factors (i.e., HES and HEY family members); however, the genome contains tens of thousands of putative RBPJ binding sites, and NICDs regulate a diverse array of genes in a cell type/tissue-specific context (58). Thus, as a first step toward defining the gene regulatory network underlying neural crest-to-mural cell differentiation, we used Notch3 ChIP-seq to identify cis-regulatory elements (CREs) directly bound by N3ICD in N3ICD-GFP-transduced cultures. In principal component analysis based on all Notch3 peaks (called by comparison of Notch3 IP and matched input controls), N3ICD-GFP-transduced cells clustered distinctly from control GFP-transduced cells along principal component 1, which explained 71% of the variance (
In RNA-seq differential expression analysis of GFP+ mural cells and neural crest, the average fold change of genes associated with N3ICD-enriched peaks exceeded that of non-enriched peaks (
hPSC Maintenance
Matrigel-coated plates were prepared by resuspending a frozen 2.5 mg aliquot of Matrigel, Growth Factor Reduced (Corning, Glendale, Ariz.) in 1 mL of DMEM/F12 (Life Technologies, Carlsbad, Calif.) and diluting the resulting solution in 29 mL of DMEM/F12. 1 mL of this solution was used to coat each well of five 6-well plates. Plates were stored at 37° C. for at least 1 h prior to use, and up to 1 week. The following hPSC lines were used: H9 hESCs (77) (WiCell, Madison, Wis.); IMR90-4 iPSCs (78) (WiCell); DF19-9-11T iPSCs (79) (WiCell); WTC11 iPSCs (80) (Gladstone Institutes, San Francisco, Calif.). hPSCs were maintained at 37° C., 5% CO2 on Matrigel-coated plates in E8 medium (STEMCELL Technologies, Vancouver, Canada) with daily medium changes. When hPSCs colonies began to touch, cells were dissociated as colonies using ˜7 min of Versene (Life Technologies) treatment and transferred to a new Matrigel-coated plate at a split ratio of 1:12.
Neural crest was differentiated according to a previously established protocol (38, 39). When hPSC colonies began to touch, 3-4 wells of cells were dissociated using ˜7 min of Accutase (Innovative Cell Technologies, San Diego, Calif.) treatment, 1 mL per well. The Accutase/single cell suspension was transferred to 4× volume of DMEM/F12 medium and cells were counted using a hemocytometer. Cells were centrifuged for 5 min at 200×g. The cell pellet was resuspended in 1 mL of E8 medium and a volume of the resulting suspension containing 2.84×106 cells transferred to a tube containing 6.5 mL E8 medium supplemented with 10 μM ROCK inhibitor Y-27632 (Tocris, Bristol, United Kingdom). The resulting cell suspension was distributed to 3 wells of a Matrigel-coated 6-well plate, 2 mL per well. Cells were incubated at 37° C., 5% CO2. The following day, differentiation was initiated by changing medium to E6-CSFD medium. E6-CSFD medium is E6 medium prepared according to ref. (81) supplemented with 1 μM CHIR 99021 (Tocris), 10 μM SB431542 (Tocris), 10 ng/mL FGF2 (Waisman Biomanufacturing, Madison, Wis.), 1 μM dorsomorphin dihydrochloride (Tocris), and 22.5 μg/mL heparin sodium salt from porcine intestinal mucosa (Sigma-Aldrich, St. Louis, Mo.). E6-CSFD medium was replaced daily for 15 days. Cells were passaged when confluent: one well of cells was dissociated with 1 mL of Accutase for ˜5 min. The Accutase/single cell suspension was transferred to 4× volume of DMEM/F12 medium and centrifuged for 5 min at 200×g. The cell pellet was resuspended in 600 μL of E6-CSFD medium and 100 μL of the resulting suspension transferred to each of 3-6 wells of a 6-well plate each containing 2 mL E6-CSFD medium (for a split ratio of 1:6).
On day 15, 3-6 wells of neural crest cells were dissociated using ˜5 min of Accutase treatment, 1 mL per well. The Accutase/single cell suspension was transferred to 4× volume of DMEM/F12 medium and cells were counted using a hemocytometer. Cells were centrifuged for 5 min at 180×g, 4° C. MACS buffer was prepared by supplementing Dulbecco's phosphate-buffered saline, no calcium, no magnesium (Life Technologies) with 0.5% bovine serum albumin (Sigma-Aldrich) and 2 mM ethylenediaminetetraacetic acid (Sigma-Aldrich). The cell pellet was resuspended in 60 μL MACS buffer per 107 cells. FcR Blocking Reagent, human (Miltenyi Biotec, Auburn, Calif.) and Neural Crest Stem Cell Microbeads, human (Miltenyi Biotec) were added to the cell suspension at 20 μL each per 107 cells. Cells were incubated for 15 min at 4° C. Cells were sorted through an LS Column in a MidiMACS Separator (Miltenyi Biotec) according to manufacturer protocols. Briefly, the column was primed with 3 mL MACS buffer, cells were loaded onto the column, the column was washed 3 times with 3 mL MACS buffer, the column was removed from the MidiMACS Separator, and the cells were eluted with 5 mL MACS buffer. The eluate was centrifuged for 5 min at 180×g, 4° C. and sorted through another LS Column. Cells in the eluate were counted using a hemocytometer. The eluate was centrifuged for 5 min at 180×g, 4° C. The resulting cell pellet was resuspended in a volume of E6-CSFD medium required to achieve a concentration of 105 cells/mL. The resulting cell suspension was distributed to Matrigel-coated 6-well plates, 2 mL per well. For some experiments, Matrigel-coated 12-well plates (1 mL cell suspension per well), 24-well plates (500 μL cell suspension per well), or 48-well plates (250 μL cell suspension per well) were used. Cells were incubated at 37° C., 5% CO2.
On D15 of the neural crest differentiation, two aliquots of 106 cells were transferred to conical tubes prior to MACS and kept on ice until MACS was complete. 106 cells from the final MACS eluate were also transferred to a conical tube. These three cell suspensions were centrifuged for 5 min at 180×g, 4° C. One pre-MACS cell pellet and the post-MACS cell pellet were each resuspended in 100 μL DPBS containing 0.2 μL p75 antibody and 0.2 μL HNK-1 antibody (Table 1). The other pre-MACS cell pellet was resuspended in 100 μL DPBS containing the mouse IgG1 isotype control antibody and the mouse IgM isotype control antibody (Table 1) at concentrations matched to the corresponding p75 and HNK-1 antibodies. Samples were incubated for 30 min on ice, washed by adding 2 mL DPBS, and centrifuged for 5 min at 180×g, 4° C. Each cell pellet was resuspended in 100 μL DPBS containing 1:500 goat anti-mouse IgG1 Alexa Fluor 647 antibody and 1:500 goat anti-mouse IgM Alexa Fluor 488 antibody. Samples were incubated for 30 min on ice protected from light, washed by adding 2 mL DPBS, and centrifuged for 5 min at 180×g, 4° C. Cell pellets were fixed in 500 μL 4% paraformaldehyde (Electron Microscopy Sciences, Hatfield, Pa.) for 15 min at room temperature protected from light. Samples were centrifuged for 5 min at 180×g, resuspended in 300 μL DPBS, transferred to 5 mL flow cytometry tubes, and analyzed on a FACSCalibur flow cytometer (BD Biosciences, San Jose, Calif.) with excitation at 488 nm and 635 nm, Alexa Fluor 488 emission detected with a 530/30 filter and Alexa Fluor 647 emission detected with a 661/16 filter. FlowJo software (BD Biosciences) was used for analysis.
aApplication: FC, Flow cytometry; ICC, immunocytochemistry; WB, Western blotting; IP, immunoprecipitation; ChIP: chromatin immunoprecipitation
The lentiviral plasmids pWPI (Addgene plasmid #12254), psPAX2 (Addgene plasmid #12260), and pMD2.G (Addgene plasmid #12259) were obtained from Addgene (Watertown, Mass.) as gifts from Didier Trono. To generate pWPI-N3ICD, we amplified a cDNA fragment encoding the intracellular domain of Notch3 from a cDNA library generated from hPSC-derived neural crest. This fragment spans nucleotides 5,074-7056 of NCBI Reference Sequence NM_000435.3, corresponding to amino acids 1,662-2,321 of NP_00426.2. To generate pWPI-N1ICD, we amplified a cDNA fragment encoding the intracellular domain of Notch1 from the neural crest cDNA library. This fragment spans nucleotides 5,522-7,930 of NM_017617.5, corresponding to amino acids 1,754-2,556 of NP060087.3. For N3ICD and N1ICD, the forward primers (Table 2) contained a Kozak consensus sequence and start codon; forward and reverse primers (Table 2) included PacI restriction enzyme sites. To generate pWPI-TBX2, we amplified the TBX2 coding sequence from pcDNA3.1-TBX2 (NCBI Reference Sequence NM_005994.4) (GenScript, Piscataway, N.J.). The forward primer (Table 2) contained a Kozak consensus sequence; forward and reverse primers (Table 2) included PacI restriction enzyme sites. pWPI and the resulting PCR fragments were digested with PacI. Ligation was performed with Instant Sticky-end Ligase Master Mix (New England Biolabs, Ipswich, Mass.), and resulting products transformed into NEB Stable Competent E. coli (New England Biolabs). Single ampicillin-resistant colonies were picked and PCR screened for presence of insert using primers annealing to the EF-1α promoter and IRES (Table 2). Sanger sequencing was used to identify clones with forward-oriented inserts. pWPI, pWPI-N3ICD, pWPI-N1ICD, and pWPI-TBX2 plasmids were expanded and purified using the EndoFree Plasmid Maxi Kit (Qiagen, Germantown, Md.).
293TN cells (System Biosciences, Palo Alto, Calif.) were maintained on uncoated 6-well plates in DMEM (Life Technologies) supplemented with 10% fetal bovine serum (Peak Serum, Wellington, Colo.), 1 mM sodium pyruvate (Life Technologies), and 0.5× GlutaMAX Supplement (Life Technologies). When 293TN cells reached 90% confluence, psPAX2 (1 μg/well), pMD2.G (0.5 μg/well), and pWPI or pWPI-N3ICD or pWPI-N1ICD or pWPI-TBX2 (1.5 μg/well) were cotransfected using FuGENE HD Transfection Reagent (9 μL/well) (Promega, Madison, Wis.). Medium was replaced 16 hours after transfection, and virus-containing supernatants collected 24, 48, and 72 hours later. Supernatants were filtered through a 0.45 μm filter and concentrated 100× using Lenti-X Concentrator (Takara Bio, Mountain View, Calif.).
aPrimers target 3’UTR and thus do not amplify transgene-derived transcripts
bFrom ref. (103)
When neural crest cells reached ˜40-50% confluence (˜2-3 days post-MACS), lentiviral transduction was performed by replacing medium in each well E6-CSFD medium containing 30-50 μL N3ICD-GFP, N1ICD-GFP, or TBX2-GFP lentivirus per mL, or 5-8 μL GFP (control) lentivirus per mL, which achieved transduction efficiencies of 50-80%. E6-CSFD medium was replaced every other day for 6 days. In some experiments, culture medium was supplemented with 10 μM CB-103 (MedChemExpress, Monmouth Junction, N.J.). The resulting cultures were either used directly for analysis or sorted to isolate GFP+ and GFP− cells as described below.
RNA extraction was performed using the RNeasy Plus Micro Kit (Qiagen). Cells were lysed with 350 μL Buffer RLT supplemented with 1% β-mercaptoethanol (Sigma) and transferred to gDNA Eliminator spin columns. 350 μL 70% ethanol was added to each lysate, and lysates were loaded onto RNeasy MinElute spin columns. Columns were washed with Buffer RW1, Buffer RPE, and 80% ethanol according to manufacturer protocols. RNA was eluted with RNase-free water and concentration quantified using a NanoDrop 2000 spectrophotometer (Thermo Scientific, Waltham, Mass.). 250-1000 ng of RNA was reverse-transcribed for 1 h at 37° C. using the OmniScript RT Kit (Qiagen) and 1 μM Oligo(dT)12-18 primers (Life Technologies). 1 U/μL RNaseOUT (Life Technologies) was included in the reverse-transcription reactions. Reaction products were diluted to 10 ng/μL. 20 μL qPCR reactions were carried out with 10 ng cDNA and 500 nM each forward and reverse primers (Table 2) using PowerUp SYBR Green Master Mix (Life Technologies) and an AriaMx Real-Time PCR System (Agilent Technologies, Santa Clara, Calif.). An annealing temperature of 60° C. was used for all reactions.
Cells were washed once with DPBS and lysed with Cell Lysis Buffer (Cell Signaling Technology, Danvers, Mass.) supplemented with 1× Halt Protease Inhibitor Cocktail (Thermo Scientific). Lysates were sonicated with three 5 s pulses at 40% power with a ⅛-inch probe and centrifuged at 4° C. for 5 min, 14,000×g. Supernatants were transferred to new tubes and protein concentrations quantified using the Pierce BCA Protein Assay Kit (Thermo Scientific). Lysates were diluted with lysis buffer to 1 mg/mL. 420 μl of each lysate was precleared by adding 40 μl of prewashed Protein A Magnetic Beads (Cell Signaling Technology) and incubating with rotation for 20 min at room temperature. Beads were removed using a magnetic separation rack. To reduce nonspecific adsorption of DNA to magnetic beads, DNA was fragmented by adding 2 μl (2000 U) micrococcal nuclease to each lysate and incubating for 30 min at 37° C. Digestion was stopped by adding 10 μl of 0.5 M EDTA to each lysate. A 20 μl aliquot of each lysate was removed and stored at −80° C. to serve as a 10% input control. The remaining 400 μl of each lysate was split between two new tubes, and Notch3 or isotype control antibody (at matched concentration, Table 1) added. Lysates were incubated with rotation overnight at 4° C. 20 μl of prewashed Protein A Magnetic Beads were added to each lysate and incubated with rotation for 20 min at room temperature. Beads were pelleted using a magnetic separation rack, supernatant removed, and beads washed with 500 μl of lysis buffer. This step was repeated for a total of 5 washes. After the final wash, beads were pelleted, supernatant removed, and beads resuspended in 20 μl of Western blot sample buffer. 20 μl Western blot sample buffer was also added to each 10% input sample. All samples were heated at 95° C. for 5 min. Beads were pelleted via centrifugation and resulting supernatants and 10% input samples processed for anti-RBPJ Western blotting as described below, except a mouse anti-rabbit IgG conformation-specific secondary antibody (Table 1) was used for detection.
Cells were lysed with radioimmunoprecipitation assay (RIPA) buffer (Rockland Immunochemicals, Pottstown, Pa.) supplemented with 1× Halt Protease Inhibitor Cocktail and centrifuged at 4° C. for 5 min, 14,000× g. Supernatants were collected, transferred to new tubes, and protein concentrations quantified using the Pierce BCA Protein Assay Kit. For each sample, ˜20 μg of protein was diluted to equal volume with water, mixed with sample buffer, and heated at 95° C. for 5 min. Samples were resolved on 4-12% Tris-Glycine gels and transferred to nitrocellulose membranes. Membranes were blocked for 1 h in tris-buffered saline plus 0.1% Tween-20 (TBST) supplemented with 5% non-fat dry milk. Primary antibodies (Table 1) were diluted in TBST supplemented with 5% non-fat dry milk and were added to membranes and incubated overnight at 4° C. on a rocking platform. Membranes were washed five times with TB ST. Secondary antibodies (Table 1) were diluted in TBST supplemented with 5% non-fat dry milk and were added to membranes and incubated for 1 h at room temperature on a rocking platform, protected from light. Membranes were washed five times with TBST and imaged using an Odyssey 9120 (LI-COR, Lincoln, Nebr.). Band intensities were quantified using Image Studio software (LI-COR).
Fluorescence-Activated Cell Sorting (FACS) and Post-FACS Culture 6 days after lentiviral transduction, cells were dissociated using ˜30 min of Accutase treatment, 1 mL per well. The Accutase/single cell suspension was transferred to 4× volume of DMEM/F12 medium and centrifuged for 5 min at 200×g. The cell pellet was resuspended in MACS buffer supplemented with 2 μg/mL 4′,6-diamidino-2-phenylindole (DAPI; Life Technologies). A FACSAria III Cell Sorter (BD Biosciences) was used to isolate DAPI− GFP+ cells (live, N3ICD-overexpressing cells) and DAPI−GFP− cells (live, non-overexpressing cells). Excitation was at 405 nm and 488 nm, with DAPI emission detected with a 450/50 filter and GFP emission detected with a 502LP dichroic and 530/30 filter. Cells from a non-transduced well were used as a gating control. The resulting cell suspensions were centrifuged for 5 min at 200×g, 4° C. Cell pellets were resuspended in E6 medium and seeded on Matrigel-coated plates at 2×104 cells/cm2. Medium was replaced daily.
Cells were washed once with DPBS and fixed with 4% paraformaldehyde for 15 min. Cells were washed three times with DPBS and blocked/permeabilized with DPBS supplemented with 10% goat serum (Life Technologies) and 0.1% Triton-X100 (Sigma-Aldrich) for 1 h at room temperature. Primary antibodies (Table 1) diluted in DPBS supplemented with 10% goat serum were added to cells and incubated overnight at 4° C. on a rocking platform. Cells were washed three times with DPBS. Secondary antibodies (Table 1) diluted in DPBS supplemented with 10% goat serum were added to cells and incubated for 1 h at room temperature on a rocking platform, protected from light. Cells were washed three times with DPBS. Cells were incubated for 5 min in DPBS supplemented with 4 μM Hoechst 33342 (Life Technologies). Images were acquired using an Eclipse Ti2-E epifluorescence microscope (Nikon, Tokyo, Japan) with a 20× objective.
RNA-seq was performed on cells from the H9, IMR90-4, DF19-9-11T, and WTC11 hPSC lines. For each line, differentiation-matched samples of neural crest cells, and GFP− and GFP+ cells isolated via FACS 6 days after transduction of neural crest with N3ICD-GFP lentivirus, were analyzed. Neural crest cells were dissociated with Accutase for ˜5 min. The Accutase/single cell suspension was transferred to 4× volume of DMEM/F12 medium and centrifuged for 5 min at 200×g, 4° C. FACS was performed as described above; resulting GFP− and GFP+ populations were centrifuged for 5 min at 200×g, 4° C. Supernatants were aspirated and the resulting cell pellets immediately lysed with Buffer RLT Plus (Qiagen) supplemented with 1% β-mercaptoethanol and frozen at −80° C. RNA extraction was performed using the RNeasy Plus Micro Kit (Qiagen). Lysates were thawed on ice, processed through gDNA Eliminator spin columns, processed through RNeasy MinElute spin columns per manufacturer instructions, and eluted into RNase-free water.
RNA quality control, library preparation, and sequencing were performed by Novogene (Sacramento, Calif.). RNA quantity was assessed using a NanoDrop spectrophotometer; RNA quality was assessed using an Agilent 2100 Bioanalyzer. Poly(A) mRNA enrichment was performed using poly(T) oligo-conjugated magnetic beads, first-strand cDNA synthesis performed using random hexamer primers, second-strand cDNA synthesis performed, and libraries prepared using the NEBNext Ultra II RNA Library Prep Kit for Illumina (New England Biolabs). Libraries were sequenced on a NovaSeq 6000 (Illumina, San Diego, Calif.) with approximately 20 million 150 bp paired-end reads obtained for each sample.
A DNA sequence from lentiviral transfer plasmid pWPI extending from the PacI site to the 3′ end of the WPRE (containing the IRES and eGFP CDS) was added to the reference genome (hg38) to permit quantification of transgene-derived transcripts. RNA-seq FASTQ files from the experiment described above and from the literature (obtained from the Gene Expression Omnibus, Table 3) were aligned to the resulting reference genome using STAR (version 2.5.3a) (82). Gene-level counts were generated using the featureCounts function from Subread (version 2.0.3) (83). Transcripts per million (TPM) were calculated using gene lengths derived from featureCounts as previously described (35).
Transcriptome comparison between hPSC-derived brain pericyte-like cells, GFP+ cells from this work, and in vivo human brain pericytes was performed for protein-coding genes (based on the list at genenames.org/download/statistics-and-files). Data for in vivo brain pericytes were obtained from a previous meta-analysis of single cell RNA-seq studies (36). In this meta-analysis, a mock bulk RNA-seq dataset was constructed from each source dataset (84-88) by (i) averaging gene counts across the pericyte cluster, (ii) obtaining the subset of protein-coding genes, and (iii) generating mock TPM values by normalizing total counts to 106. Bulk RNA-seq TPM values from hPSC-derived brain pericyte-like cells (from the literature) and GFP+ cells (this work) were similarly re-normalized to 106 after obtaining the subset of protein-coding genes. To generate the scatterplots
Raw counts from featureCounts were input to DESeq2 (version 1.32.0) (89) for differential expression and principal component analyses. The DESeq2 variance stabilizing transformation was used to generate counts data for input to principal component analysis and hierarchical clustering. Hierarchical clustering on genes and samples (one minus Pearson correlation with average linkage) was performed using Morpheus (software.broadinstitute.org/morpheus/). Differential expression analysis was performed using the DESeq2 Wald test with Benjamini-Hochberg correction. The DESeq2 design included differentiation (hPSC line) matching as described above. Genes with adjusted P-values <0.05 were considered differentially expressed. Gene Set Enrichment Analysis (version 4.2.3) (90) was performed using DESeq2-normalized counts for neural crest and GFP+ cell samples. GSEA was performed with gene set permutation and otherwise default settings. Genes enriched in GFP+ cells compared to neural crest were tested against the KEGG (91) and gene ontology-biological processes (GO-BP, (92)) databases (version 7.5.1). Gene sets with false discovery rates (FDR)<0.05 were considered enriched. Visualization of reads aligned to the human genome was performed using Integrative Genomics Viewer (version 2.5.0).
Analysis of single cell RNA-seq data from developing mouse brain (93) was performed in Scanpy (94) (version 1.9.1). The loom file containing expression data and metadata was obtained from the authors' website (Table 3). Clusters annotated as neural crest and mesenchymal cell types by the authors were selected for analysis. A complete list of the authors' ClusterName identifiers is shown in
Decellularization was performed 6 days after transduction of neural crest cultures in 12-well plates with GFP or N3ICD-GFP lentiviruses as described above. The decellularization protocol was adapted from ref (95). The following buffers were pre-warmed to 37° C.: DPBS, Wash Buffer 1 (100 mM disodium phosphate, 2 mM magnesium chloride, 2 mM EDTA, pH 9.6), Lysis Buffer (8 mM disodium phosphate, 1% Triton X-100, pH 9.6), Wash Buffer 2 (10 mM disodium phosphate, 300 mM potassium iodide, pH 7.5). Cells were washed twice with 1 mL DPBS and three times with 1 mL Wash Buffer 1. Cells were incubated with 1 mL Lysis Buffer for 15 min at 37° C. Lysis Buffer was replaced with 1 mL fresh Lysis Buffer; cells were incubated for 1 h at 37° C. Lysis Buffer was replaced with 1 mL fresh Lysis Buffer; cells were incubated for an additional 1 h at 37° C. Lysis Buffer was removed and the resulting extracellular matrix washed 3 times with 1 mL Wash Buffer 2 and 4 times with 1 mL water. Water was removed and 250 μL RIPA buffer added. Extracellular matrix was scraped from the bottom of the well. The resulting solution was transferred to a microcentrifuge tube and sonicated with two 10 s pulses at 40% power with a ⅛-inch probe. Protein concentration in the resulting solution was quantified using the BCA assay. For normalization of total protein to cell number, cells from a parallel well of the 12-well plate were dissociated using Accutase and counted using a hemocytometer.
The coculture cord formation assay was performed 5 days after isolation of GFP+ and GFP− cells via FACS from a N3ICD-GFP-transduced culture as described above. 8-well chamber slides were coated with Matrigel, growth factor reduced, at 250 μL per well. Matrigel was allowed to gel at 37° C. for 1 h. HUVECs (American Type Culture Collection, Manassas, Va.) maintained in EGM-2 medium (Lonza, Walkersville, Md.), were dissociated using a ˜15 min treatment with 0.25% trypsin-EDTA (Gibco). The resulting cell suspension was transferred to a 4× volume of DMEM supplemented with 10% FBS. Neural crest cells, GFP+ cells, and GFP− cells were dissociated using 5-15 min of Accutase treatment and the resulting cell suspensions were transferred to 4× volumes of DMEM/F12 medium. Cells were counted using a hemocytometer and centrifuged for 5 min at 200×g. Supernatants were removed and cell pellets resuspended in 1 mL EGM-2 medium. For the HUVEC-only control, HUVEC cell suspension and EGM-2 medium were combined to yield a suspension containing 2.2×104 HUVECs per 500 μL. For the coculture conditions, HUVEC cell suspension, coculture cell suspension (neural crest, GFP+, or GFP− cell suspension), and EGM-2 medium were combined to yield suspensions containing 2.2×104 HUVECs and 6.6×104 coculture cells per 500 μL. 500 μL of the resulting cell suspensions were added to the prepared wells of the 8-well chamber slides. Phase contrast and GFP images were acquired after 24 h and 72 h using an Eclipse Ti2-E microscope with a 4× objective.
To assess the ability of extracellular matrix from GFP- and N3ICD-GFP-transduced cells to support endothelial cord formation, neural crest cultures in 48-well plates 6 days post-transduction with GFP or N3ICD-GFP lentiviruses were decellularized. The decellularization protocol was as described above, except all wash and incubation steps performed using 200 μL of solution, and the protocol terminated after the final wash with water. This procedure was also performed on parallel cell-free wells to serve as a no-extracellular matrix control. Additional parallel wells were coated with 200 μL Matrigel, Growth Factor Reduced, which was allowed to gel at 37° C. for 1 h. 2.75×104 HUVECs in 250 μL EGM-2 medium were added to each well. Phase contrast images were acquired 16 h after addition of HUVECs using an Eclipse Ti2-E microscope with a 4× objective. Cells were subsequently fixed and processed for VE-cadherin immunocytochemistry as described above. To quantify the extent of cord formation, blinded phase contrast images were scored on the following 4-point scale. 0: No cords apparent. 1: Few cords apparent, most cells not associated with cords. 2: Many cords apparent, most cells associated with cords. 3: Virtually all cells associated with cords.
Calcium imaging was performed 6 days after transduction of a neural crest cultures with N3ICD-GFP lentivirus as described above. FLIPR Calcium 6 dye (Molecular Devices, San Jose, Calif.) was prepared according to manufacturer instructions. 500 μL of prepared dye was added to the existing 500 μL of culture medium and cells incubated at 37° C., 5% CO2 for 2 h. The plate was transferred to a microscope environmental chamber at 37° C., 5% CO2 and equilibrated for 30 min. Images were acquired every 5 s for 300 s using an Eclipse Ti2-E microscope with a 4× objective. At t=50 s, a 1:114 dilution of saturated KCl solution (4.56 M, for a final concentration of 40 mM) was added to the well. ImageJ was used to quantify mean fluorescence intensity Ft at each time point and data are displayed as ΔF/F=(Ft−F0)/F0.
To assess function of KATP channels, cells 6 days after transduction with GFP or N3ICD-GFP lentiviruses were labeled with FLIPR Calcium 6 dye as above, and 20 μM pinacidil (Santa Cruz Biotechnology, Dallas, Tex.) or DMSO added 1.5 h after addition of dye. After an additional 30 min incubation, the plate was transferred to the microscope environmental chamber. Images were acquired every 5 s for 60 s and 40 mM KCl added at t=20 s. Mean fluorescence intensity was quantified as above.
The contraction assay was performed 2 days after isolation of GFP+ cells via FACS from a N3ICD-GFP-transduced culture as described above. The plate was transferred to a microscope environmental chamber at 37° C., 5% CO2 and equilibrated for 30 min. At t=0 min, a 1:114 dilution of saturated potassium chloride solution, or an equivalent volume of water, was added to the culture medium and the plate briefly rocked to mix. Phase contrast images were acquired immediately upon addition of potassium chloride or water and 15 min thereafter using an Eclipse Ti2-E microscope with a 20× objective. The Freehand Selection Tool in ImageJ was used to trace the outlines of 16 cells per 20× field at times 0 and 15 min, and the Measure function used to obtain A0 and A15, the cell areas at times 0 and 15 min, respectively. For each cell, the percent change in area was computed as (A15−A0)/A0×100%. These values were averaged across the 16 cells in each field to generate the values shown in
ChIP-seq was performed on cells 6 days after transduction of neural crest cultures with GFP and N3ICD-GFP lentivirus as described above. Three independent differentiations were performed, with average transduction efficiency of GFP-transduced cultures 82±9% GFP+ and N3ICD-GFP-transduced cultures 87±3% GFP+. Cells were dissociated with Accutase and transferred to DMEM/F-12. Crosslinking was performed with 1% formaldehyde for 10 min and the reaction quenched with glycine. Cells were centrifuged for 5 min at 2,000×g, 4° C. Supernatants were removed and cell pellets stored at −80° C. Nuclei isolation and chromatin digestion with micrococcal nuclease were performed using the SimpleChIP Enzymatic Chromatin IP Kit (Magnetic Beads) (Cell Signaling Technology) according to manufacturer protocols. 50 μl of resulting chromatin preparation from a GFP-transduced sample was subject to crosslink reversal and DNA purification to confirm appropriate digestion and estimate chromatin concentration. Approximately 60 μg of chromatin was used for each immunoprecipitation. Samples were diluted to 500 μL and Notch3 antibody (Table 1) added. Samples were incubated overnight with rotation at 4° C. Antibody-bound fragments were isolated using Protein G magnetic beads. Resulting chromatin samples and matched 10% input control samples were subject to crosslinks reversal and DNA purification using the SimpleChIP Enzymatic Chromatin IP Kit, per manufacturer protocols. DNA quality control, library preparation, and sequencing were performed by Novogene. Libraries were sequenced on a NovaSeq 6000 with approximately 30 million 150 bp paired-end reads obtained for each sample.
Sequencing reads were aligned to the human genome (hg38) using bowtie2 (version 2.2.1) (96). Sambamba (version 0.8.2) and bedtools (version 2.30.0) were used to remove unmapped reads, reads mapped to blacklist regions (using the database available at https://github com/Boyle-Lab/Blacklist) (97), and reads mapped to decoys and nonchromosomal assemblies. Peakcalling was performed with MACS (version 3.0.0a7) (98), using IP and matched input control samples, paired-end mode, and a P-value cutoff of 0.0005. DiffBind (version 3.2.7) (59) calling DESeq2 (89) was used to identify peaks enriched in N3ICD-GFP-transduced samples compared to GFP-transduced samples (adjusted P-value <0.05, DESeq2 Wald test with Benjamini-Hochberg correction). ChIPseeker (version 1.28.3) (99) was used for peak annotation. DeepTools (version 3.5.1) (100) was used to generate bigWig files and peak profile plots. MEME-ChIP (https://meme-suite.org/meme/tools/meme-chip, version 5.4.1) (101) was used for motif enrichment analysis. Genome browser visualizations were created using the UCSC Genome Browser (102).
Individual wells of cultured cells that underwent identical experimental treatments are defined as replicates. Details of replication strategy are provided in figure legends. Student's unpaired or paired t tests were used for comparison of means from two experimental groups. One-way analysis of variance (ANOVA) was used for comparison of means from three or more experimental groups. Two- or three-way ANOVA was used for comparison of means and blocking of differentiation-based variability if data from multiple differentiations were combined (one/two factors being the experimental treatment(s) and one factor being the differentiation). Following ANOVA, Dunnett's post-hoc test was used for comparison of multiple treatments to a single control, or Tukey's honest significant difference (HSD) test was used for multiple pairwise comparisons. For cord formation score data, the nonparametric Kruskal-Wallis test was used followed by the Steel-Dwass test for multiple pairwise comparisons.
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This patent application claims the benefit of priority of United States Provisional Patent Application No. 63/246,238 filed on Sep. 20, 2021, which is incorporated herein by reference in its entirety.
This invention was made with government support under NS103844 awarded by the National Institutes of Health. The government has certain rights in the invention.
| Number | Date | Country | |
|---|---|---|---|
| 63246238 | Sep 2021 | US |
