Resident mesenchymal vascular progenitors modulate adaptive angiogenesis and pulmonary remodeling via regulation of canonical Wnt signaling.

Adaptive angiogenesis is necessary for tissue repair, however, it may also be associated with the exacerbation of injury and development of chronic disease. In these studies, we demonstrate that lung mesenchymal vascular progenitor cells (MVPC) modulate adaptive angiogenesis via lineage trace, depletion of MVPC, and modulation of β-catenin expression. Single cell sequencing confirmed MVPC as multipotential vascular progenitors, thus, genetic depletion resulted in alveolar simplification with reduced adaptive angiogenesis. Following vascular endothelial injury, Wnt activation in MVPC was sufficient to elicit an emphysema-like phenotype characterized by increased MLI, fibrosis, and MVPC driven adaptive angiogenesis. Lastly, activation of Wnt/β-catenin signaling skewed the profile of human and murine MVPC toward an adaptive phenotype. These data suggest that lung MVPC drive angiogenesis in response to injury and regulate the microvascular niche as well as subsequent distal lung tissue architecture via Wnt signaling.

ATP‐binding cassette super‐family G member 2

cigarette smoke exposure

multidrug resistance

Mesenchymal vascular progenitor cells

pulmonary hypertension

room air

receptor tyrosine kinase inhibitor, SU5416

vascular endothelial growth factor

wild‐type

stabilized β‐catenin

INTRODUCTION

Loss and dysfunction of pulmonary microvasculature has been implicated in the decreased alveolar gas exchange area in emphysema, a major manifestation of chronic obstructive pulmonary disease (COPD). Recent evidence highlighted a role for microvascular pathology in both the early pathogenesis and heterogeneity of the disease. , , , , However, the mechanisms by which changes in the microvasculature underlie the development of chronic lung diseases remain unresolved. To date, studies have primarily focused on endothelial cell injury as the basis for microvascular dysfunction during the development of emphysema, while lung resident mesenchymal cell types and adaptive angiogenesis have been largely overlooked. We, therefore, tested the hypothesis that lung mesenchymal vascular progenitor cells (MVPC) modulate adaptive angiogenesis and pulmonary tissue remodeling via regulation of canonical Wnt/β‐catenin signaling. MVPC may, therefore, contribute to the development of emphysema by altering the homeostatic maintenance of the microvascular niche.

Adaptive angiogenesis occurs in response to tissue hypoxia, injury, and during wound healing. However, this de novo angiogenesis, while reparative in nature, can also become maladaptive if not patterned correctly via remodeling, regression, and pruning. , , Mesenchymal regulation of pulmonary vasculogenesis and angiogenesis in the distal lung have been well‐characterized during development. , , Recently, lineage analysis using a lung‐specific enhancer coupled to the mesenchymal restricted transcription factor Tbx4 provided evidence for mesenchymal‐derived angiogenic precursors. , MVPC have since been lineage labeled and characterized in adult murine lung during both tissue homeostasis and disease. , , , Their perivascular localization and communication , would predict crosstalk between MVPC and components of the lung microvasculature during health and distal lung injury resulting in emphysema.

In this report, using murine and human models, we described a vital role of resident lung MVPC as multipotent vascular progenitors in maintaining the integrity of the distal lung during homeostasis and adaptive angiogenesis in response to injury. These studies also defined how disease specific increases in canonical Wnt/β‐catenin signaling by MVPC influenced adaptive angiogenesis within the lung microvascular niche.

MATERIALS AND METHODS

Study approval

The Institutional Animal Care and Use Committee at National Jewish Health or Vanderbilt University approved all animal procedures and protocols. These studies utilized banked patient cell lines obtained using IRB #9401 approved by the Vanderbilt University Medical Center IRB Committee, Nashville, TN, USA. Patients were consented under this IRB for the generation and storage of human cell lines. Primary cells were obtained from advanced COPD patients (GOLD C or D) with severe physiological impairment (FEV1/FVC < 0.7 and FEV1% Pred < 30%) requiring lung transplantation as previously described. ,

Study design

Isolated human and murine MVPC and murine in vivo age matched models were utilized. Endpoint analysis was performed in a blinded fashion. Sample size and number of replicates are specified in the figure legends, methods, and Supporting Table S1. We have previously reported that the recombination efficiency, at two alleles, is approximately 50% and that recombination with GFP expression strongly correlated with Abcg2 (Supporting Figure S2B‐F).

Isolation and characterization of primary lung MVPC

Human lung plastic adherent cells were isolated from explant lung tissue post autopsy or transplant by collagenase digest (Vanderbilt IRB Protocol 9401) to form a suspension. The cells were stained with antibodies to sort CD45neg ABCG2pos cells (lung mesenchymal progenitors) using a BD FACSAria III (BD Biosciences, San Jose, California). Techniques were previously described and ABCG2 was validated as a cell surface marker for both murine eGFP labeled and human MVPC. , Antibodies for flow cytometry were purchased form eBiosciences, (San Diego, CA) or Thermo Fisher (Waltham, MA). A summary of human lung mesenchymal progenitor line expression of cell surface determinants is presented in Supporting Tables S3 and S4.

Murine lung mesenchymal progenitors were isolated from induced ABCG2 CreERT2 × mT/mG mice using a BD FACSAria III (BD Biosciences, San Jose, California) to identify eGFP positive cells. Isolated cells were plated on attachment factor‐coated dishes, expanded, and analyzed at passage 7 to characterize CFUF and cell surface determinants as previously described. , Following expansion, all primary human and murine mesenchymal progenitors were analyzed by flow cytometry to confirm the presence of CD105, CD106, CD73, ScaI, CD44 and the absence of c‐kit, CD14, and CD45 (Supporting Table S4) using a BD Fortessa or LSRII (BD Biosciences, San Jose, California). Following cell sorting, CD45neg GFPneg or CD45negGFPpos populations were centrifuged to make cytospins for analysis (Wescor Cytopro). To compare relative growth characteristics of mesenchymal progenitors and colony forming unit‐fibroblast colonies (CFU‐F), cells were counted and diluted to a concentration of 6 × 103/mL. After colonies were formed, spent medium was removed and cells washed once with DPBS. About 4% of paraformaldehyde was used to fix the cells for 20 minutes. Following a PBS wash, Giemsa stain (Sigma Aldrich, Saint Louis, MO; Cat# GS500) was added to cover cells overnight. Giemsa stain was then removed, and the plates gently washed with water (Supporting Figure S5E).

Genetic manipulation of murine ABCG2pos mesenchymal progenitor cells (MVPCs)

ABCG2‐CreERT2 mice, a generous gift of Dr B. Sorrentino (St. Jude Children's Research Hospital, Memphis, TN), were crossed to a fluorescent eGFP reporter (Cg)‐Gt(ROSA)26Sortm4(ACTB‐tdTomato,‐EGFP) JAX stock# 007676; designated mT/mG) strain to facilitate lineage analysis and quantitation via eGFP expression. A third gene was crossed into the mice to stabilize βcatenin(Catnbloxp(Δex3) a generous gift of Dr MM Taketo (Kyoto University, Kyoto, Japan). To knockout MVPC in vivo, we crossed the Abcg2 driver/reporter strain to a mouse containing a floxp stop allele regulating the expression of Diphtheria toxin A , (JAX stock# 009669). Mice were injected intraperitoneally at 8‐10 weeks of age with a low dose (0.5mg) tamoxifen (T‐5648; SIGMA, St. Louis MO) in sesame oil, or sesame oil alone (vehicle control). , The mice were randomized and distributed as 3‐5 mice per cage for studies. These model systems, as well as isolated MVPC, were validated as previously described.

Phenotyping of pulmonary vascular dysfunction

Elevated pulmonary artery pressure was documented indirectly by the measurement of right ventricular systolic pressure (RVSP) as previously described. RVSP was measured at the time of harvest. , The number of subjects per group was 6‐8. Histologic endpoints included muscularization and microvessel density of the distal microvessels by immunostaining to detect smooth muscle actin (SMA; Dako clone 1A4) or Factor 8 (A0082 DAKO) on 6‐8 mice per group. The average inter‐alveolar distance was assessed by quantification of MLI in lungs inflated with agarose under constant temperature and pressure as described. , H&E‐stained lung sections from 6 to 8 wild‐type or transgenic mice were analyzed. For each pair of lungs, 40 histological fields were photographed and evaluated in a blinded fashion. Immunofluorescent staining was performed to lineage trace eGFP‐labeled lung mesenchymal progenitors and localize smooth muscle alpha (SMA), reagents outlined in Supporting Tables S6 and S7. Quasi‐static mechanical properties of the lung we measured using the flexiVent invasive plethysmography system (SciREQ, Inc) as previously described. , ,

Cigarette smoke exposure and Stereology

Mice were exposed to cigarette smoke for four hours daily, five days a week for 1 month. To expose the mice to cigarette smoke, two 70 mL puffs per minute from research cigarettes (University of Kentucky, 3R4F) were generated by a smoking machine (SIU24 system; Promech, Vintrie, Sweden), and then, diluted with fresh air and delivered to whole body exposure chambers. The mice were subjected to a mixture of both mainstream and side stream smoke. The total particulate matter (TPM) concentration in the chamber was kept at 100 mg/m3 at all times. , The TPM was determined by gravimetric analysis of filter samples taken during smoke exposure. Blood carbon monoxide levels in these mice were below 10%. To analyze changes in distal lung structure, images of H&E stained lung sections were taken on a Nikon Eclipse 80i microscope using NIS Elements AR software (version 4.13). A minimum of 6 non‐overlapping images were taken at 20x to avoid large vessels or airways. Images were then loaded into an interactive macro within Metamorph Software (version 7.5.0.0) for analysis. MLI and MCL were calculated from the average of all the images and the surface to volume ratio was calculated as 4 × Sum of line Intercepts/130.87 × Sum of ends.

RNA scope

RNA scope was performed using the Advanced Diagnostics HybEZII system with the RNAscope Multiplex Fluorescent Reagent Kitv2 assay per manufacturer instructions. Probes included GFP (cat# 400281) and Abcg2 (510101).

Western blot analysis

Protein extracts were made by scraping cells in RIPA buffer (Cell Signaling, Boston, MA; cat # 9806S) containing protease and phosphatase inhibitors (ThermoFisher Scientific, Waltham, MA; cat # 78444). After determination of protein concentrations and standardization, cell lysates were mixed with an equal volume of Laemmli SDS loading buffer, resolved on 10% of polyacrylamide‐SDS gels, and transferred to PVD membranes. The blots were blocked with phosphate‐buffered saline (PBS) containing 5% of dry milk and 0.1% of Tween 20, and then, treated with antibodies that detect the target proteins as labeled in the figures overnight at 4°C. The blots were washed and subsequently treated with appropriate secondary antibodies conjugated to horseradish peroxidase. After the blots are washed, specific immune complexes were visualized with SuperSignal West Pico Chemiluminescent Substrate (Supporting Table S7).

Spheroid assay & quantitation

Confluent MVECs were serum starved with medium containing 0.5% of FBS for 1 hour, then, treated with 10 µg/mL low density lipoprotein conjugated to Alexa Fluor 594 (ThermoFisher L35353) in regular culture medium. After incubation, cells were rinsed twice with PBS before passaging for spheroid formation. A micro‐mold (MicroTissues Inc #24‐906) was used to create a 2% of agarose three‐dimensional petri dish containing 96 individual recesses, which allow cells to self‐assemble into spheroids. 3D petri dishes were pre‐treated with 1 mL of culture medium for 45 minutes (3 treatments of 15 min each) prior to cell seeding in a 24 well plate. MVECs were mixed at a 3:1 ratio with GFP+ MVPCs and seeded into the 3D dish at a density of 500 cells per well in 75 µL total volume per the manufacturer's recommendation. Cells were allowed to settle for 30 minutes before adding 1 mL of medium to the area surrounding the micro‐mold. Cells were then cultured for 24 hours, during which time spheroid formation was observed. Spheroids were collected by aspirating the medium surrounding the 3D petri dish, and squirting 500 µL of pre‐warmed medium into the mold to dislodge spheroids. Spheroid‐containing medium was collected into a 15 mL conical tube and centrifuged for 5 minutes at 110 g. Supernatant was aspirated, and spheroids were resuspended in a solution of 2 mg/mL rat tail collagen (Gibco A10483‐01) combined with an equal volume of 0.5% 4000 cP methylcellulose solution (Sigma M0512) in medium. Spheroids were then pipetted in 1 mL volumes to a new 24 well plate and incubated for 30 minutes to polymerize the collagen before adding 100 µL of culture medium to each well. After 24 hours, spheroids were imaged on a Keyence BZ‐X810 digital fluorescent microscope. BZ‐X800 analysis software was used to measure the migratory radius of cells around the spheroid.

Single cell RNA sequencing

Approximately 4000 ABCG2 eGFP labeled cells were captured and single‐cell RNA sequencing libraries were prepared using the 10x Genomics Chromium 3′ v3 platform. Libraries were sequenced on an Illumina NovaSeq 6000 (paired‐end; read 1:28 cycles, read 2:100 cycles) to an average depth of >120 000 reads per cell. RNA sequencing reads were processed and aligned to the mouse genome (mm10) using the Cell Ranger pipeline (v3.0.2) from 10x Genomics. Analysis was performed using the Loupe Cell Browser v. 3.1.1 10x Genomics.

Optical coherence microscopy

A custom‐built optical coherence microscopy (OCM) system was used for ex vivo imaging. A 0.2 obstruction‐to‐pinhole ratio (diameter‐to‐diameter) annular aperture was used to generate a Bessel beam to increase OCM depth‐of‐field. The aperture dimensions were tuned to optimize depth‐of‐field while minimizing complex conjugate artifacts. All images were acquired with a 0.1 NA 10x PLAN objective (Leica). Lateral resolution and depth‐of‐field were 1.8 and 106 μm, respectively. OCM data were collected using a custom‐built spectrometer with a superluminescent diode light source (889 ± 93 nm bandwidth, Superlum) detected at 70 kHz line‐rate using a 4096 pix. CMOS array (Basler). Axial resolution was 2.1 μm in air and system SNR was 94 dB with 900 μW on the sample. All volumetric data sets were acquired over a 1 × 1 mm field‐of‐view with 1000 × 1000 A pixels in 14.6 s. Individual OCM volumes were dispersion compensated and cropped to only retain in‐focus depths. OCM images were acquired at 5 random fields in each of the nine optically cleared lungs (5 control, 4 disease). Custom MATLAB code was used to quantify en face projections of each OCM volume using OCM contrast as a surrogate for vasculature. The images were first binarized using a threshold set 5 times above the standard deviation of the noise floor. Microvascular regions were then manually segmented and total vascular density in each region was calculated as the ratio between total pixels with and without signal. One‐sided two‐sample t test of unequal variances shows statistically significant differences in mean vascular density between control and disease animals (P < .005, alpha = 0.05).

Electrical cell‐substrate impedance sensing (ECIS)

Human lung MVECs (Lonza, Walkersville) were plated at a concentration of 112 500 cells per well on gelatin coated 8W1E PET ECIS culture ware arrays (Applied Biophysics, Troy) overnight to achieve confluence. The following day, MVPCs were added at a concentration of 37 500 cells per well. Prior to experiments the optimal concentration of MVEC and ratio of MVPC was determined. MVPC lines were normalized by cell number. Controls for these experiments included untreated MVEC and MVEC with wounding. On the third day, the arrays were put on the ECIS ZTheta, Applied Biophysics (Troy, NY). Resistance recordings were performed at 4 kHz every 10 minutes over 24 hours. At 2‐3 hours, an electrical wound was created by administering a 20 second pulse at 60 000 Hz. In some cases, the pulse was immediately repeated to ensure cell death. In other experiments not including MVPC, a total 150 000 MVEC were applied per well and allowed to adhere overnight. Recovery from wounding in all experiments was normalized to the first resistance value data collected subsequent to wounding. These experiments were performed with two sample replicates and repeated twice.

Transcriptome analysis

Array analysis and qRT‐PCR was performed as described, , in triplicate or with an n of three or greater independent patient samples. Briefly, total RNA was prepared with Qiagen RNA Isolation Kit reagents (Qiagen, Valencia, CA) for total RNA isolation and analysis of gene expression. qRT‐PCR assays were performed in triplicate and levels of analyzed genes were normalized to hypoxanthine phosphoribosyltransferase abundance (GAPDH or HPRT; primer list is provided in Supporting Table S6). Complimentary DNA generated from amplified RNA was hybridized to duplicate Affymetrix (Santa Clara, CA) Human Gene 1.0 ST arrays. Microarray analysis was carried out using Bioconductor version 3.2 (R 3.2.2). The oligo package was used to read in and normalized the data with RMA. The moderated t test implemented in the limma package was used for differential expression testing. Genes that were significantly upregulated or downregulated (P < .05) and showed an expression fold change of at least 1.7‐fold greater or lesser than control samples were used for further analyses. Normalized expression values for these genes are represented in a heatmap. Further, the corresponding gene names were queried against the STRING database (http://string‐db.org/, accessed December 10, 2015) to explore the protein‐protein interactions. PathVisio 3.2.1. was used to schematically represent and annotate the relevant functional association network of differentially expressed genes. The raw array data and normalized matrix is available under the GEO accession GSE94060.

Quantitation of collagen

About 10 fields of view per two sections, four sections per mouse of trichrome stained mouse lungs were photographed at 20x‐40x mag. Resulting color images were scanned to quantitate the number and intensity of blue (collagen) positive pixels relative to red. n = 7‐8 per group. Images were scanned using Fiji (Image J; version 2.0.0‐rc‐43/1.51a) using a custom plug in written by M. Majka (Denver, CO). The tool was written in the ImageJ macro language to detect pixels with a blue intensity over a desired threshold. This macro set all pixels that had the desired blue intensity to the color yellow and outputs a count of the number of yellow pixels. The specified threshold limit was based on a positive and negative control image.

Imaging

Epifluorescent and brightfield images were captured with Nikon Eclipse 90i upright epifluorescence or Nikon Eclipse TS100 using the Nikon DS‐Fi1 camera with NIS elements AR 4.11.00 acquisition software. The BZ‐X800 KEYENCE system, with capture and analysis software, was also used. Two photon imaging was performed as previously described. Fluorochromes used included DAPI (to label nuclei), secondary antibodies conjugated to Alexa 488 or Alexa 594 (ThermoFisher, Hampton, NH) to detect antibodies outlined in Supporting Table S7.

Statistical analysis

Data were analyzed by one‐way ANOVA followed by Tukey's HSD post‐hoc analysis. Murine qPCR and patient samples were analyzed using nonparametric Wilcoxon/Kruskal Wallis and a chi square approximation. All analyses used JMP version 9.0.2. Data presented as ± standard error from the mean (±SEM). Significance was defined as P‐value <.05*, P‐value <.01** or P‐value <.001***.

RESULTS

MVPC are an essential constituent of distal lung tissue structure

Abcg2, the multidrug resistance (MDR) transporter largely responsible for the side population (SP) phenotype of cells, has been used by our group and others to enrich for putative progenitor cells in many adult tissues in various species. , , , , , , , , To localize the lineage labeled MVPC in the three‐dimensional tissue structure, precision‐cut lung slices (PCLS) were imaged using two‐photon microscopy (Figure 1A‐C). The imaging depicts that MVPC have multiple long processes in the alveolar‐capillary regions (LINK to MOVIE). To further define the nature of the Abcg2 MVPC, single cell RNA sequencing was performed. A single cell suspension of murine lung tissue was sorted to separate eGFP expressing cells (Figure 1D). Transcriptomes of 4017 CD45neg eGFP cells were sequenced to a mean of 315 576 reads/cell (a median of 953 genes per cell) using the 10xGenomics platform. Using the 10xGenomics Loupe Cell Browser, we determined that 96% of CD45neg eGFP cells expressed a transcriptome indicative of multipotent mesenchymal vascular progenitors (Figure 1E,F and Table 1). Key determinants included Ly6a (ScaI), Flk1, Flt1 Cdh5, Tek (Tie2), Eng (CD105), Pecam (CD31), Foxf1, Lyve1, Itga1, Edn1, S1pr1, and BMPR2 (Table 1; Supporting Figure S1). , , , , Additionally, this population lacked significant expression of Car4, Dll4, , , demonstrated expression of c‐Kit and the angiogenic molecule CD93 (Supporting Figure S1). Hierarchical clustering and GO analysis was performed and identified categories associated with angiogenic processes (Figure 1F and Supporting Table S2) including: regulation of endothelial barrier, endothelial cell development (including lymphatic), lung vasculature development/morphogenesis, vasculogenesis, sprouting angiogenesis and positive regulation of cell or endothelial cell migration, regulation of BMP signaling pathway, response to hypoxia, and mesenchyme development. Categories associated with epithelial regulation were: lung alveolus development, branching morphogenesis of an epithelial tube and positive/negative regulation of epithelial cell differentiation and migration (Supporting Table S2). In vitro three‐dimensional vascular spheroid co‐culture analysis demonstrated the tube forming and migratory potential of murine MVPC relative to lung MVEC (Figure 1G,H). Thus, MVPC play a regulatory role in the lung microvascular niche, comprise a multipotent vascular progenitor phenotype as well as directly participate in adaptive angiogenesis.

FIGURE 1

Isolated Abcg2pos MVPC have angiogenic transcriptional signatures and potential. A‐C, Abcg2‐Cre‐ERT2 Rosa26mTmG WT mice were induced with intraperitoneal tamoxifen. Two days post induction mice were sacrificed, and lungs agarose inflated using constant pressure, to obtain lung tissue for precision cut lung slices for two‐photon imaging. Membrane labeled eGFP MVPC were visible in green and mTomato lung tissue was detected in the red channel. A, Representative 2 µM section through the lung tissue Z stack. B and C, Reconstruction of the three‐dimensional lung image naïve and with a Gaussian filter. Scale and grid dimension = 20 µM. D, Abcg2‐Cre‐ERT2 Rosa26mTmG WT mice were induced with intraperitoneal tamoxifen. Two days post induction mice were sacrificed, and lung tissue digested to a single cell suspension for cell sorting to obtain the eGFP labeled cells. E, t‐SNE plot depicting CD45neg eGFP labeled cells analyzed using 10x single cell RNA sequencing. F, GO clustering analysis. G and H, Angiogenic sprouting and migration potential of MVPC was defined by co‐culture three‐dimensional spheroid assays

TABLE 1

Top 50 genes in GFPpos cells

Gene	Log2 Fold Change	P‐value	Gene	Log2 Fold Change	P‐value
Scgb1a1	−7.223871011	1.44E‐107	Itga1	5.409905416	6.08E‐25
Ptprb	6.421083773	9.79E‐33	Fmo1	5.418503357	6.22E‐25
Calcrl	6.311036351	1.34E‐31	Scn7a	5.622690678	8.43E‐25
Tmem100	6.196069716	7.24E‐31	Icam2	5.434842991	1.38E‐24
Cdh5	6.114112411	5.51E‐30	Sema3c	5.404884676	2.12E‐24
Cxcl12	6.098934754	2.82E‐29	Egfl7	5.061042323	2.97E‐24
Tspan7	6.1222942	3.30E‐29	Thbd	5.145866085	8.66E‐24
Clec14a	6.128228101	3.30E‐29	Ace	5.064925166	8.83E‐24
Cldn5	5.793411224	7.32E‐29	Adgrf5	4.904596787	3.27E‐23
Plvap	6.032582526	8.18E‐29	Cd93	4.950572449	6.13E‐23
Ramp2	5.834408603	1.01E‐28	Slco2a1	5.021742097	7.85E‐23
Aqp1	5.911595357	1.29E‐28	Esam	5.107124152	7.95E‐23
Tie2/Tek	6.244118402	2.09E‐28	Sca1/Ly6a	4.759290772	3.16E‐22
Eng	5.962395401	2.35E‐28	Bmpr2	4.778387384	4.01E‐22
Lyve1	6.433252167	6.94E‐28	Edn1	5.021552994	5.60E‐22
Foxf1	6.024244291	5.74E‐27	Acvrl1	4.73362789	6.45E‐22
Pecam1	5.630994125	5.82E‐27	Sparcl1	4.897329011	1.11E‐21
Gpihbp1	5.803532867	7.70E‐27	Ctla2a	4.736117235	1.22E‐21
Tm4sf1	5.55159617	1.19E‐26	S1pr1	4.708281041	4.84E‐21
Ly6c1	5.646064165	1.23E‐26	Cavin1	4.737835792	5.87E‐21
Cyyr1	5.603486745	4.69E‐26	Id3	4.619945449	7.65E‐21
Efnb2	5.775305044	5.70E‐26	Id1	4.723059956	9.32E‐21
Hmcn1	5.763531721	9.67E‐26	Vwf	4.949834686	1.02E‐20
Hpgd	5.40633778	1.26E‐25	Flt1	4.574584046	1.08E‐20
Cav1	5.319645308	3.29E‐25	Pltp	4.510079688	1.51E‐20

To define a functional significance for the lung MVPC population, we selectively depleted these cells in vivo by engineering mice, in which Abcg2‐Cre‐ERT2 was crossed to and a reporter Rosa26mTmG. , Mice were administered a single dose of tamoxifen (0.02 mg/g) and lung tissue sections were then analyzed for changes in tissue architecture. Distal alveolar simplification was evident 1 month following MVPC depletion and demonstrated by the presence of increased mean linear intercept (MLI) and decreased fractional lung volume in the absence of detectable pulmonary hypertension as assessed by Fulton Index (Figure 2A‐D; Supporting Figure S2A). About 15 months following MVPC depletion loss of distal lung structure was exacerbated and resembled an emphysematous‐like phenotype (Figure 2E,F). The increased mean linear intercept was associated with increased compliance and decreased resistance (Figure 2G‐I). Thus, targeted depletion of Abcg2 lineage labeled MVPC negatively impacted distal lung structure, suggesting they are required for the maintenance of distal lung parenchymal structure.

FIGURE 2

Targeted depletion of MVPC effect on distal lung structure and adaptive angiogenesis. WT or f/fSTOP DTA Abcg2‐Cre‐ERT2 Rosa26mTmG mice were induced with intraperitoneal tamoxifen. One month or 15 months following induction mice were sacrificed, and lungs agarose inflated using constant pressure, to obtain lung tissue for histological and immunofluorescent analyses. n = 4,5 (1 month). A, Quantitation of MLI. B, Fractional volume, the fraction of an image that is occupied by lung tissue. C and D, Representative H&E stained lung tissue sections. Scale bar = 50 µM. n = 10, 12 (15 months) E and F, Representative H&E stained lung tissue sections. Scale bar = 100 µM. G. Quantitation of MLI. H and I, Mean compliance and resistance measured by FlexiVent. WT, f/fSTOP DTA mice were induced with intraperitoneal tamoxifen, 2 weeks later mice were exposed to cigarette smoke for four weeks. Six weeks following induction mice were sacrificed, and lungs agarose inflated using constant pressure, to obtain lung tissue for histological analyses. n = 4, 9, 4, 5. K, Quantitation of MLI and L, surface to volume ratio. Immunostaining was performed on lung tissue sections to detect smooth muscle alpha actin (SMA) and F8 positive microvessels as well as muscularization. M‐O, The immune‐positive microvessels were counted per field of view. A 6‐8 sections of 20 field of view (f.o.v.) per section were evaluated

To address the role of Abcg2 MVPC in the maintenance of distal lung structure, we exposed WT and MVPC depleted mice to one month of cigarette smoke (CSE). Neither WT nor DTA mice demonstrated an increase in MLI or mean surface to volume ratio (Figure 2J,K) relative to the room air (RA) baseline. However, WT mice responded to CSE with adaptive vascular remodeling characterized by increased microvessel density and muscularization, which was not detected in the DTA mice (Figure 2L‐N; 0‐50 µM; Supporting Figure S2G‐I). These data highlight two pivotal findings, that adaptive microvascular remodeling preceded loss of distal lung tissue structure and that MVPC are required for adaptive angiogenesis in response to injury.

Activation of Wnt signaling in MVPC is sufficient to cause emphysema‐like distal lung remodeling and exacerbate vascular Injury

Chronic lung diseases, including emphysema, are associated with abnormal regulation of developmental signaling cascades, including Wnt/β‐catenin. , , We previously demonstrated that activation of canonical Wnt signaling in murine MVPC promoted microvascular dysfunction. Therefore, to assess whether activation of Wnt/β‐catenin signaling in MVPC would exacerbate the emphysematous loss of tissue structure, we employed an endovascular injury model in mice using the vascular endothelial growth factor (VEGF) receptor tyrosine kinase inhibitor, SU5416 (Sugen) in combination with hypoxia exposure. , , VEGF, a proangiogenic and survival factor for endothelial and mesenchymal cells, , , is decreased in COPD in spite of hypoxemia. While Sugen hypoxia could affect multiple cell types, similar to the elastase and other models of emphysema, , the predominant effect is on the vasculature, specifically lung endothelium. Thus, inhibition of VEGF receptor signaling in combination with hypoxia exposure is complex and results in significant endothelial injury, apoptosis, apoptosis resistant cells , , , , and is a significant contributor to the development of COPD/emphysema and pulmonary hypertension (PH). Additionally, this vascular injury model, differs from smoke in that there is not an initiating inflammatory cascade, the phenotype is a result of a direct vascular injury. Thus, the model was well suited to examine how MVPC modulate the microvascular niche to maintain lung structure and function.

Wnt signaling was activated in MVPC by crossing the Abcg2‐Cre‐ERT2 driver strain with a floxed Δexon 3 allele of β‐catenin, thereby expressing an inducible β‐catenin lacking degradation domains. , The lungs of stabilized β‐catenin (βOE) lineage labeled mice were compared to wild‐type (WT). Lungs were harvested from a standard three‐week model of Sugen with hypoxia exposure and compared to room air (RA) vehicle, RA + Sugen or hypoxia vehicle groups in age matched mice. We found that in response to hypoxia WT mice exhibited predicted responses with increased RVSP, muscularization, and microvessel density (Figure 3A‐C). WT mice responded to Sugen + hypoxia, with increased RVSP and characteristic decreased muscularization and microvessel density (Figure 3A‐C). Wnt activation in the MVPC significantly increased RVSP in response to Sugen following both RA and hypoxia exposure, while the muscularization and microvessel density were not significantly changed from baseline (Figure 3A‐C). In fact, βOE mice exhibited decreased muscularization and microvessel density overall, closely resembling the loss of microvessels by WT mice exposed to Sugen + hypoxia (Figure 3B,C; Supporting Figure S3 and S4). Overall, in contrast to WT, Wnt activation in MVPC blunted the adaptive responses to hypoxia including RVSP and microvessel density. Interestingly, the baseline number of collagen positive microvessels was greater in the βOE lungs vs WT (Figure 3D, Supporting Figure S3D‐I). Finally, in the lungs of βOE mice exposed to hypoxia + Sugen, significant findings included decreased microvessel density with increased total collagen content (Figure 3E), areas of subpleural fibrosis (Figure 3F) and MLI (Figure 3G‐K). Interestingly, comparing isolated WT to βOE MVPC in a spheroid sprouting angiogenesis assay, the βOE MVPC demonstrated increased tube forming and migratory capacity relative to the WT MVPC (Figure 3L‐N). Thus, the microvascular phenotype resulting from abnormal Wnt activation in MVPC coupled to endovascular injury was associated with the appearance of an emphysematous––like phenotype and enhanced perivascular and interstitial fibrosis, thus, exacerbation of injury. These data illustrate the importance of regulated Wnt signaling by MVPC in the maintenance of pulmonary microvascular and alveolar architecture.

FIGURE 3

Canonical Wnt activation in Abcg2pos MVPC blunted adaptive responses to hypoxia and exacerbated injury following Sugen‐hypoxia exposure. Adult WT or βcatenin over expresser (βOE) mice were treated with intraperitoneal tamoxifen. Two weeks following induction mice were grouped for exposure to room air (RA) + CMC vehicle (Veh.), room air + Sugen5416 (SU5416), hypoxia + CMC vehicle (10% oxygen; HY Veh.) or hypoxia + SU5416 (HY SU). Histological and physiological parameters were analyzed after three weeks. A, A pressure transducer was placed in the jugular to the right heart to measure RVSP. Lungs were agarose inflated using constant pressure to obtain lung tissue for histological and immunofluorescent analyses. Immunostaining was performed on lung tissue sections to detect (B) smooth muscle alpha actin (SMA) and (C) F8 positive microvessels as well as muscularization. The immune‐positive microvessels were counted per field of view. A 6‐8 sections of 20 field of view (f.o.v.) per section were evaluated. D, Trichrome staining was performed on tissue sections and collagen positive microvessels were enumerated. A 6‐8 sections of 20 f.o.v. per section were examined. E, Total collagen per f.o.v. was also calculated using FIJI software. F, Representative image of fibrosis in a trichrome stained βOE hypoxia + SU5416 lung section. G‐J, Representative trichrome images illustrate distal lung tissue structure. Scale bars = 100 µM. K, MLI was calculated to evaluate simplification of distal lung tissue structure. Data presented as the mean (±SEM). n = 6‐9 mice/group. RA Vehicle (white box); RA SU5416 (light grey box); HY Vehicle (dark grey box); HY SU5416 (black box).L‐N, Angiogenic sprouting and migration potential of primary eGFPpos MVPC was defined by co‐culture three‐dimensional spheroid assays (n = 10, 10)

MVPC directly participate in adaptive microvascular remodeling

Given the marked effect of MVPC on endothelial and vascular function that indicates significant intercellular or paracrine crosstalk, and the difference in sprouting capacity of βOE MVPC, we next performed lineage analysis to evaluate the spatial fate of MVPC in response to vascular injury and remodeling. In both WT and βOE mouse strains, there was evidence of intravascular localization of MVPC following Sugen + hypoxia exposure (Figure 4A,L), as well as close proximity of MVPC with microvessels, especially in regions of bridging and sprouting angiogenesis (Figure 4B,C). In Sugen + hypoxia injured lung tissue eGFP labeled the βOE MVPC lineage derived cells that formed SMAneg structures, resembling microvessels in the distal lung (Figure 4D‐I). Many of these structures contained DAPI positive nuclei in their lumen (*), suggesting continuity with the pulmonary circulation. Only the βOE Sugen + hypoxia group developed focal areas of interstitial fibrosis (Figure 4E‐G). Further analysis of the structures was performed to identify endothelial investment. Factor VIII or podoplanin was used to distinguish capillary vs lymphatic structures. Factor VIII colocalization with eGFP demonstrated that while some MVPC are present adjacent to capillary microvessels, eGFPPOS vascular like structures did not exhibit a capillary endothelial‐lined lumen (Figure 4G‐I). Podoplanin is expressed by both lymphatic endothelium and alveolar Type 1 cells, however, it is typically used to discern lymphatic from capillary endothelium in the mouse. Podoplanin and eGFP co‐localization demonstrated that MVPC did not co‐express podoplanin and that subgroups of both WT and βOE MVPC derived vascular structures had a lymphatic endothelial lined lumen (Figure 4J‐O). Uninjured and control groups were presented in Supporting Figures S4 and S5. MVPC contributed to the genesis of vascular‐like structures, however, lacking expression of capillary and lymphatic endothelium.

FIGURE 4

MVPC directly participate in de novo angiogenesis following lung injury. Immunostaining was performed on lung tissue sections from room air (RA) + CMC vehicle (Veh.), room air + Sugen5416 (SU5416), hypoxia (10% oxygen) or hypoxia + SU groups to detect eGFP labeled MVPC and lineage derivatives. Costaining was performed to detect SMA positive muscularized vessels, Factor VIII (F8; G&I) or podoplanin (podopln; J‐O) positive microvascular endothelium. Representative images from WT or βOE hypoxia + SU groups were presented. A, MVPC migrate along vascular wall. B‐D, MVPC form vascular structures via bridging or sprouting adjacent to SMApos microvessels. E‐I, Fibrosis was identified in the βOE hypoxia + SU groups. E, Trichrome staining. F, Immunofluorescent detection of eGFP and SMA. G, Enlarged from F, Immunofluorescent detection of eGFP, SMA, and FactorVIII. H, Enlarged eGFP expressing vascular structure from G. I. Enlarged eGFP F8 negative vascular structure from G, H. J, Immunofluorescent detection of eGFP and podoplanin in WT lungs. K, Enlarged eGFP expressing structures adjacent to podoplanin positive endothelium from J. L, Migrating MVPC do not express podoplanin. M, Immunofluorescent detection of eGFP and podoplanin in βOE lungs enlarged in N and O. N, eGFP adjacent to podoplanin positive endothelium. O, eGFP positive structures lacking podoplanin expressing endothelium. Nuclei are stained with DAPI (blue). The presence of nuclei in MVPC derived structures was indicated by the presence of *. n = 6‐9 mice/group. Scale bars = 100 µM

Deregulated expression of an angiogenic profile by COPD MVPC

Following the observation that the lung MVPC played a crucial function in the maintenance of the alveolar architecture, we hypothesized that the gene expression profile of MVPC from COPD patients would exhibit alterations to their angiostasis repertoire. Human MVPC were isolated from explanted lung tissue via ABCG2 enrichment and characterized as previously described, expressing mesenchymal cell surface determinants, lacking hematopoietic, and endothelial determinants as well as forming colonies (CFU‐F) (Supporting Tables S3‐S5, Supplemental Figure S6E‐F). , , Global gene expression profiling with hierarchical clustering and GO analysis was performed (Figure 2A; Supporting Figure S6A‐D, Supporting Table S5). GO categories associated with angiogenic processes and increased gene expression included: circulatory/cardiovascular system development, vasculature development/morphogenesis, angiogenesis, and positive regulation of cell or endothelial cell proliferation. GO categories associated with angiogenic processes that showed decreased gene expression included: negative regulation of cell proliferation and circulatory/cardiovascular system development. Categories associated with epithelial remodeling that showed increased gene expression were: regulation of epithelial cell migration and proliferation.

Targeted analysis of gene expression by PCR defined distinct changes in Wnt signaling, AXIN2, PROX1, SFRP1, DKK1, LRP6 by COPD MVPC, as well as the noncanonical ligand WNT5A, relative to healthy, indicating that Wnt/β‐catenin signaling is upregulated in MVPC (Figure 5B). These findings are in contrast to endothelial and epithelial cells from COPD patients, in which Wnt signaling is decreased. , , The Wnt modulators WLS and CREB5 were also decreased in COPD MVPC. Genes associated with modulation of the actin cytoskeleton and migration were also changed between groups. SVIL decreased while EDNRA and HMMR increased (supervillain, endothelin receptor, hyaluronan mediated motility receptor/CD168) in COPD MVPC (Figure 5C). The ligand, SLIT2, which influences angiogenesis and directional migration also increased in COPD MVPC, while it's receptor, ROBO1, was unchanged. , Most notably, expression of angiopoietin 1 (ANGPT1) was decreased in COPD MVPC suggesting that microvessel stability was impaired. Western blot analysis of normal and COPD MVPC lysates further confirmed higher levels of protein expression of DKK1, WNT5A, and SLIT2 compared to healthy MVPC (Figure 5D). Differentially regulated and interacting signaling pathways were identified using STRING analysis and included canonical Wnt, Robo‐Slit, angiopoietins1/2‐Tie2/TEK, FGF, TGFβ, BMP, and NOTCH (Figure 5B,C; Supporting Figure S6G; Supporting Table S5). Further analysis demonstrated that Wnt activated murine MVPC recapitulated the human COPD MVPC differential expression of Dkk1, Prox1, Angpt1, Slit2 as well as Wnt5a (Figure 5F relative to B). Murine Wnt activated MVPC also expressed significantly increased levels of Angpt2, further suggesting microvessel stability was impaired. A comparative summary of gene expression was presented in Figure 5G. Together these results suggest that under the control of Wnt signaling, MVPC regulate cell fate, proliferation, migration, and angiogenesis.

FIGURE 5

Disrupted Wnt signaling in ABCG2pos COPD MVPC disrupts MVEC function. A, Heatmap for differentially expressed genes in MVPC from COPD vs non‐diseased lungs (color scale shown at the top right) B and C, Validation of representative genes expressed in COPD ABCG2pos lung MVPC, compared to control, enriched in GO categories of B, Wnt signaling and C, actin binding, contractility, and migration. The mean of combined patient samples per group as well as results for individual samples are presented. n = 3‐6 patient samples per group. D, Western blot analysis of Dkk1, Wnt5a and Slit2 protein expression. n = 3, 3. Data presented as the mean ± standard error of mean (SEM). E, Cocultures of pulmonary MVEC and MVPC were analyzed for the effect of control or COPD MVPC on barrier function following injury. MVPC were plated on a monolayer of MVEC at a ratio of 3:1. The groups underwent no injury or an electrical wounding injury using the ECIS system. The presence of COPD MVPC following injury decreased the rate at which barrier formation is recovered. Quantitation of normalized resistance at indicated time points (Δ) was presented in bar graph format. Data presented as mean (±SEM). Controls included MVEC alone and uninjured MVEC. n = 4. F, Murine WT and Wnt activated βOE MVPC were analyzed by PCR to examine the expression of angiogenic transcripts identified as different between control and COPD samples. n = 3, 3. All amplification was normalized to a housekeeping gene and the results presented as mean fold change over control. Data presented as mean ± SEM. G. Representative summary of murine and human PCR data

We next tested the direct effects of COPD MVPC on MVEC migration and barrier function in a model of wound injury and repair using an electrical cell‐substrate impedance sensing (ECIS) system. The ability of cells to migrate into the denuded area and close the monolayer, as measured by increased resistance, is an indication of structural and functional activity of MVEC. Loss of barrier function and migration are necessary for angiogenesis and repair, whereas the formation of tight junctions and barrier integrity indicate vessel stability. , , , , MVPC were co‐cultured with a confluent monolayer of MVEC, which was disrupted using an electrical “wounding” injury (Figure 5E). The rate at which the MVEC barrier formation was recovered following injury was indicated by the slope of change in transcellular resistance relative to that at the time of injury. The rate of MVEC barrier function recovery was decreased by addition of COPD MVPC following injury, compared to addition of healthy MVPC or MVEC alone (Figure 5E). These data support the hypothesis that COPD MVPC decreased MVEC barrier function and may negatively modulate microvascular stability.

The lung vasculature has evolved highly responsive mechanisms to maintain tissue perfusion and oxygen homeostasis. Our data suggest that in response to lung and vascular injury, Wnt signaling in the novel Abcg2HI subset of MVPC regulate adaptive responses of the microvasculature including: angiogenesis vs microvessel rarefaction, muscularization of microvessels or collagen deposition and the MVPC direct contribution to the formation of angiogenic tubes (Figure 6). Therefore, it is reasonable to speculate that the Wnt signaling status and subsequent function of MVPC is regulated by the disease microenvironment, to influence the microvasculature program of adaptation resulting in either repair or remodeling long term.

FIGURE 6

Wnt signaling in the Abcg2HI MVPC regulate adaptive responses of the microvasculature. Wnt signaling and function of MVPC is regulated by the disease microenvironment, to influence the microvascular program of adaptation resulting in either repair or remodeling. The microvascular program of adaptation includes: angiogenesis vs microvessel rarefaction, muscularization of microvessels or collagen deposition and the MVPC direct contribution to the formation of angiogenic tubes. MVPC depicted in green and microvascular endothelial cells (MVEC) in red

DISCUSSION

Adult tissue resident vascular precursors are an elusive but important population that have been difficult to isolate and characterize in vivo due to lack of specific markers. Our studies show that Abcg2pos lung mouse adult tissue resident vascular precursors (MVPC) have a defining transcriptome, which may be useful in future studies. To study MVPC functions, we genetically depleted and lineage traced this population demonstrating that, in vivo, MVPC are necessary for adaptive microvascular remodeling following exposure to cigarette smoke as well as endovascular injury and, when MVPCs are depleted, aged mice demonstrate severe emphysema.

Results from our single cell analyses as well as three‐dimensional spheroid assays further defined the Abcg2 lineage labeled population as a multipotent adult vascular progenitor reservoir with rigorous angiogenic potential, relative to lung microvascular endothelial cells (MVEC). While MPC in the developing and adult lung are typically described as influencing epithelial cell processes during morphogenesis or as a potential origin of the myofibroblast lineage during adult tissue remodeling, our previous studies highlighted a role of ABCG2pos MVPC in the maintenance and regulation of microvascular homeostasis. The existence of these vascular progenitors was initially demonstrated by our group and others via the identification of a lung “side population” by flow cytometry, and definition that the membrane expression of Abcg2 transporter conferred this phenotype. , , , , Further identification of differentiated and progenitor mesenchymal subpopulations, and understanding of their importance in tissue remodeling has more recently been aided by single cell transcriptome analysis in adult murine models of fibrotic injury.

The function of adaptive angiogenesis is the “structural adaptation” or “angioadaptation” of the vascular network to provide adequate oxygenation to tissues in response to injury or stress. The processes of angiogenesis, vascular remodeling or regression and pruning are necessary in normal angiostasis, tissue repair/regeneration, and the pathogenesis of disease processes. The genetic depletion of MVPC decreased adaptive microvascular endothelial angiogenesis in response to cigarette smoke exposure, while Wnt activation in these cells blunted the typical pro‐angiogenic response to physiologic hypoxia in vivo. Stabilized expression of Wnt/β‐catenin in MVPC converted the cells to a proangiogenic phenotype both in vitro and in vivo, a property that exacerbated systemic endovascular injury in mice.

The appearance of mesenchymal derived angiogenic tubular structures driven by this Wnt‐dependent phenomenon and endovascular injury correlated with an exacerbated emphysema‐like phenotype, characterized by decreased microvessel density, increased MLI and interstitial fibrosis. Previously, we reported that Wnt activation in MVPC and the genesis of the derived vascular structures were associated with exacerbated fibrosis and injury in the bleomycin mouse model. In these studies, the presence of Wnt activated MVPC lineage‐derived tubes, lacking discernable endothelium, was indicative of their direct contribution to adaptive angiogenesis. The absence of these MVPC derived structures in wild‐type mice suggested a defect in vascular patterning. Although their significance is currently unclear, we speculate that the MVPC form transient structures that normally would become endothelialized to resolve injury, while in the presence of activated Wnt signaling they form stabilized structures and contribute to the development of disease. The first concept is supported by studies in bone marrow MSC in the context of wound healing where primitive vascular tubes are thought to prime the network toward the formation of new capillaries. , The second is supported by the role β‐catenin plays in adherens junctions independent of Wnt signaling. Alternatively, these incomplete vascular structures resemble tumor microcirculation and may contribute to vascular dysfunction in chronic lung diseases as they may exhibit varying levels of barrier effectiveness, which in turn influences local inflammation and remodeling. Longer term studies are necessary to understand the significance and function of these MVPC‐derived structures.

The combination of tissue simplification and fibrosis observed in our models may also be linked to a net loss of microvessel density, similar to the pathology described for pulmonary vascular disease associated with connective tissue diseases such as systemic sclerosis or combined pulmonary emphysema and fibrosis (CPEF) , or tubulointerstitial fibrosis. The severity of tissue remodeling in these instances is thought to be influenced by the presence of microvascular dysfunction or vasculopathy. , Fibrotic remodeling and chronic rejection may also be preceded by loss of microvascular integrity and density following lung transplantation. In COPD, microvascular dysfunction and loss occur not only in the lung, but also systemically, and is invoked in muscle mass wasting and cachexia, which are clinical indicators of increased mortality. ,

Chronic lung diseases, including COPD/emphysema, are associated with abnormal regulation of developmental signaling cascades, including Wnt/β‐catenin. , , , , , , , , , , Isolated human COPD MVPC exhibited active Wnt signaling. Both human COPD MVPC and murine Wnt activated MVPC expressed markers indicative of adaptive angiogenic phenotype including canonical Wnt targets Dkk1, Prox1, Wnt5A, and decreased angiopoietin 1 (Angpt1). In the presence of VEGF inhibition, the timing and level of signaling or environmental co‐factors produced by MVPC likely balance the response of the microvascular endothelium as well as repair vs remodeling. , , , This interaction may explain why in response to hypoxia the wild‐type lungs had typical increased microvascular muscularization vs perivascular collagen deposition in the Wnt activated MVPC lungs. The observation that adaptive angiogenesis in our injury models occurred prior to significant changes in distal lung structure, suggesting that deregulated microvascular patterning plays a role during the onset of tissue pathology. The role of Wnt signaling during vascular homeostasis, regression, repair and remodeling is appreciated with regard to the endothelium , as it promotes sprouting and tip cell specification with the Notch pathway and delta like ligand 4 (Dll4). , , , β‐catenin expression is regulated by hypoxia inducible factors (HIFs) and also regulates VEGF‐A and Dkk1 expression. , , , Together Wnt, VEGF and Notch regulate the balance of vascular regeneration and remodeling in response to injury, in cell‐specific and dose‐dependent manners. Together these studies support a model in which canonical Wnt signaling regulates the ability of Abcg2 MVPCs to act as vascular progenitor and also to function as regulatory cells, maintaining MVEC function and response to injury.

While VEGF signaling was targeted in these studies as a method to induce endovascular injury, specifically defining the vascular cells responsible for the phenotype is likely complicated by effects on both the endothelium and mesenchyme. Additionally, while the exacerbation of remodeling following vascular injury was demonstrated in the Wnt activated MVPC strain, the specific stimuli that initiated the cascades that led to the simplification of the distal lung microvasculature and epithelium have not been defined, highlighting a need for further evaluation. Ongoing studies in our lab are designed to better understand the complexity of MVPC function as well as how changes in MVPC signaling influence the diverse cell populations in the lung including microvascular endothelium, vascular smooth muscle, alveolar epithelium (Type 1 & 2), additional mesenchymal populations (fibroblasts, myofibroblasts, and lipofibroblasts) as well as respective progenitors. Based on these data demonstrating the negative impact of sustained Wnt activation in MVPC on the microvasculature following injury, relative to the therapeutic effect of pan activation of Wnt signaling in rodent models of experimental emphysema, it is plausible that the context of Wnt signaling, influences overall vascular outcomes.

In summary, these results demonstrated the significance of Abcg2pos MVPC in the microvascular niche and the impact of canonical Wnt signaling on the function of MVPC during angiostasis as well as adaptive angiogenesis. Thus, our model is useful to explore the basic mechanisms of the disease onset and progression. Understanding Wnt signaling in MVPC coupled to their regulation of MVEC as well as vascular smooth muscle and epithelium will be important to identify novel targets to facilitate microvascular repair and pulmonary tissue function.

CONFLICT OF INTEREST

The authors have no conflicts of interest to declare.

AUTHOR CONTRIBUTIONS

Conceptualization, S.M. Majka, M.E. Summers; Methodology, M.E. Summers, B.W. Richmond, S. Menon, R.M. Sheridan, S.A. Majka, J.A. Bastarache, J.D. West, S. De Langhe, P. Geraghty, D.J. Klemm, H.W. Chu, R.S. Friedman, Y.K. Tao, R.F. Foronjy, S.M. Majka; Investigation, M.E. Summers, B.W. Richmond, M.M. Taketo, J.A. Kropski, S. Menon, R.M. Sheridan, S.A. Majka, J.A. Bastarache, J. D. West, S. De Langhe, P. Geraghty, D.J. Klemm, H.W. Chu, R.S. Friedman, Y.K. Tao, R.F. Foronjy, S.M. Majka; Writing Original Draft, S.M. Majka, M.E. Summers, D.J. Klemm, R.F. Foronjy; Writing ‐ Review & Editing, S.M. Majka, M.E. Summers, B.W. Richmond, J.A. Kropski, J.A. Bastarache, R.F. Foronjy; Funding Acquisition, S.M. Majka; Resources, J.A. Kropski, B.W. Richmond, M.M. Taketo, Y.K. Tao, R.F. Foronjy; Supervision, S.M. Majka.

Fig S1

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Video S1

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