Regeneration of functional alveoli by adult human SOX9+ airway basal cell transplantation
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Irreversible destruction of bronchi and alveoli can lead to multiple incurable lung diseases. Identifying lung stem/progenitor cells with regenerative capacity and utilizing them to reconstruct functional tissue is one of the biggest hopes to reverse the damage and cure such diseases. Here we showed that a rare population of SOX9+ basal cells (BCs) located at airway epithelium rugae can regenerate adult human lung. Human SOX9+ BCs can be readily isolated by bronchoscopic brushing and indefinitely expanded in feeder-free condition. Expanded human SOX9+ BCs can give rise to alveolar and bronchiolar epithelium after being transplanted into injured mouse lung, with air-blood exchange system reconstructed and recipient’s lung function improved. Manipulation of lung microenvironment with Pirfenidone to suppress TGF-β signaling could further boost the transplantation efficiency. Moreover, we conducted the first autologous SOX9+ BCs transplantation clinical trial in two bronchiectasis patients. Lung tissue repair and pulmonary function enhancement was observed in patients 3–12 months after cell transplantation. Altogether our current work indicated that functional adult human lung structure can be reconstituted by orthotopic transplantation of tissue-specific stem/progenitor cells, which could be translated into a mature regenerative therapeutic strategy in near future.
Keywordslung regeneration transplantation stem cell bronchiectasis alveoli
Regeneration of human skin (Gallico et al., 1984), corneal epithelium (Rama et al., 2001; Rama et al., 2010) and hematopoietic system (Copelan, 2006) by autologous transplantation of tissue-specific stem/progenitor cell has been achieved decades ago and now has become a routine therapeutic approach. However, regeneration of large inner organs, such as lung, remains one of the biggest challenges to modern medicine. Lung-related diseases are the third-leading cause of human death globally. Most of the lethal lung diseases such as chronic obstructive pulmonary disease (COPD) (Mannino, 2002), idiopathic pulmonary fibrosis (Selman et al., 2004) and bronchiectasis (Moulton and Barker, 2012) are characterized by irreversible, progressive damage of lung tissues (alveoli and/or bronchi). Besides the mitigating treatments available, lung transplant surgery is the only solution for the exacerbated patients but its application is largely limited due to the extreme lack of donor lung as well as severe side effects resulted from immune-rejection. As a potential substitute, the transplantable artificial lung technique is promising but still in its infancy (Ott et al., 2010). Therefore, millions of patients are in urgent need of a new strategy to cure such diseases and stem/progenitor cell-based regenerative therapy is likely to be the biggest hope for them. Among all cells with clinical potential, mesenchymal stem cells (MSCs) or other stroma-derived cells are easy to obtain and handle. However, it is widely recognized that transplanted MSCs function mainly through paracrine or immunomodulatory mechanism (Meirelles Lda et al., 2009), with no evidence showing that they can reconstitute lung structure for regeneration purpose. Induced pluripotent stem cells (iPSCs) could be another source of “self” stem cells for autologous transplantation and indeed, iPSCs have been successfully coaxed to alveolar and airway lineage in vitro (Huang et al., 2014). However the capability of iPSC-derived cells to generate real lung structure and their tumorigenic risk remains to be evaluated in vivo (Kotton and Morrisey, 2014). To this end, tissue-resident progenitor cells from an adult’s own lung—if can be identified, isolated and expanded—can be a new option for transplantation therapy.
In adult rodent, different populations of lung stem/progenitor cells have been identified in last decade with capability to reconstruct lung epithelium. Most of the mouse lung stem/progenitor cells are facultative and can be induced to proliferate in response to injury as well as differentiate into one or more lung cell types (Kotton and Morrisey, 2014; Kim et al., 2005; Barkauskas et al., 2013; Hogan et al., 2014; Desai et al., 2014). More recently, we and others found a rare population of p63+/Krt5+ distal airway stem cells (DASCs), which play essential role in murine lung repair after influenza-induced acute injury (Zuo et al., 2015; Vaughan et al., 2015). However in adult human, whether there are lung cells with regenerative capacity in vivo need to be explored. Given the huge differences between human vs. mouse of their respiratory systems in terms of developmental process, lung lobulation, branching pattern and cell composition, the identity of human lung progenitor cells need to be rigorously evaluated.
In the current work, we discovered the putative adult human lung progenitor cells located at the bottom of “rugaes” in airway epithelium, with a SOX9 marker to distinguish them from other SOX9−/P63+/KRT5+ airway basal cells (BCs). From a trace amount of bronchoscopic brush-off lung tissues, we isolated SOX9+ BCs and expanded them in vitro indefinitely. SOX9+ BCs transplanted into injured immune-deficient mouse lung can regenerate functional lung epithelium with both human bronchiolar and alveolar epithelium reconstituted. Most importantly, for the first time we explored the clinical feasibility of autologous SOX9+ BC transplantation to treat two patients with chronic lung diseases. The clinical trial result is highly consistent with our observation on mouse model, and making it a solid basis for future large-scale clinical study.
Bronchoscopic isolation of clonogenic airway basal cells
We seeded one single BC onto feeder cells and grew them into one single colony which was then picked up by cloning cylinders and passaged continually. The latest passage of BC clones had gone through 50 doublings (=1015 fold expansion) in our lab. The single cell-derived BC clones and their original brush-off tissue samples were analyzed by high-throughput RNA sequencing (RNA-Seq). On average, we detected 16,230 genes and 25,223 transcripts. Thus, more than 60% of known human genes and transcripts were expressed in clonogenic BCs. Gene expression value correlation analysis showed that the clone transcriptome profiles are distinct from their original brush-off tissues, but the two clones from two independent persons share very similar transcriptome (Fig. 1E, Pearson correlation coefficient = 0.95). Single nucleotide polymorphism (SNP) analysis showed that BC clones have around 70% less polymorphism comparing to the brush-off tissues, which is in consistency with their single cell origination. High expression of BC markers (KRT5, P63, NGFR and S100A) and another putative mouse stem cell marker integrin α6β4 (Chapman et al., 2011) were observed in clones. In contrast, clonogenic BCs do not express other bronchial or alveolar lineage markers as shown by RNA-Seq and confirmed by immunostaining (Figs. 1F and S1B). Protein-protein interaction analysis of overexpressed genes indicated three major signal molecule networks including Notch1/2/3, FGF10/7 and Wnt7 ligand and their downstream components. All three signaling networks are previously known to play essential roles in embryonic lung development (Bellusci et al., 1997; Rajagopal et al., 2008; Tsao et al., 2008) (Fig. 1G). Gene ontology (GO) term analysis demonstrated critical biological processes enriched in BCs (Fig. 1H).
Clonal analysis of SOX9+ BCs
The whole brushing sampling and SOX9+ BCs cloning procedure was carried out on 15 individuals with a recovery rate of 100%. Donors are from 4 different disease categories including 5 normal healthy volunteers, 2 bronchiectasis patients, 3 chronic COPD patients, and 5 interstitial lung disease (ILD) patients with pulmonary fibrosis. The SOX9+ BCs from different categories of diseases showed no apparent difference in colony morphology (Fig. S3A) or marker expression (Fig. S3B). Their clonogenic efficiency seemed similar—but still need future investigation in much larger cohort to get statistically meaningful conclusion.
We further analyzed SOX9+ BCs at single cell resolution. 5 single cells from one person in normal group were selected at Passage 0 and expanded to Passage 1 and Passage 2. Great variation of their clonogenic capacity was observed at Passage 1 (coefficient variation = 59.9%) and Passage 2 (coefficient variation = 75.7%). Similar clonogenicity variation was observed in individuals from other disease categories and the average coefficient variation of all clones is 52.2% (Fig. S3C).
SOX9+ BCs grown on feeder cells can be transferred onto petri dish pre-coated with collagen fibers for feeder-free culture. The feeder-free cultured SOX9+ BC can also form colonies though their cell-cell contact within one colony is less tight comparing to those on feeders (Fig. 2D). The feeder-free cultured BCs are able to be passaged for at least 30 doublings with no obvious morphology change. Karyotyping indicated their stable genetic characteristics along with passaging (Fig. 2E). Quantitative analysis of progenitor markers (KRT5, P63 and SOX9) and lung epithelium lineage markers at both RNA and protein level indicated that there is no spontaneous differentiation of BCs in the culture process (Fig. 2F–H).
Xeno-transplanted SOX9+ BCs give rise to human lung in vivo
In control experiment, we found that the transplanted SOX9+ progenitors cannot incorporate into non-injured healthy mouse lung or porcine pancreatic elastase-injured mouse lung (data not shown). Also, human lung-derived fibroblast cells (data not shown) or human cervix-derived P63+/KRT5+/SOX9+ progenitor cells (Figs. 3G and S6E) can barely incorporate into injured mouse lung either. This data indicated the tissue specificity of different adult stem/progenitor cells.
Regenerated lung by SOX9+ BC transplantation contributed to mouse pulmonary function
TGF-β signaling modulates SOX9+ BC proliferation
Autologous SOX9+ BCs transplantation clinical trial in bronchiectasis patients
Bronchiectasis is a chronic lung disease radiographically characterized by permanent pathologic dilation of the small and medium-sized bronchi, which may lead to respiratory failure and eventually to death. Patients with bronchiectasis, if left untreated, will have a continual decrease of their pulmonary function. Current pharmacological strategies to treat bronchiectasis such as antibiotics, mucolytics and anti-inflammatory agents could only control the disease exacerbation but not improve the pulmonary function nor repair the damaged lung tissue (ten Hacken et al., 2007). To explore the clinical feasibility of autologous SOX9+ BC transplantation, we conducted a pilot trial aiming to treat bronchiectasis by regenerating functional human lung. The general trial protocol and the cell manufacturer (Regend Therapeutics Co.Ltd) were archived by China Food and Drug Administration (CFDA) and National Health and Family Planning Commission of China, and the trial was performed in national approved stem cell clinical research institute (Southwest Hospital) after strict ethic commission review of preclinical data (A part of but not all preclinical data was released in the current manuscript).
Two patients diagnosed as non-CF bronchiectasis were firstly enrolled for autologous SOX9+ BC transplantation on April, 2016. Both patients are men in 50s, non-smokers. Patient 1 was diagnosed as bronchiectasis 8 years ago with productive cough and dyspnea on exertion symptom, which worsens continually under regular pharmacological treatment. CT scan shows multiple bronchial cylinder dilation and patchy consolidation in his lung. Patient 2 was diagnosed as bronchiectasis and COPD decades ago, with productive cough and dyspnea on exertion symptom, which worsens continually under regular pharmacological treatment. CT scan shows multiple bronchial cystic dilation, thicken bronchial wall and patchy consolidation in his lung.
In the current study, we revealed that a small population of SOX9+ BCs in adult airway can regenerate human lung epithelium. A few SOX9+ BCs brushed off from human airways can be expanded to sufficient number in feeder-free condition and transplanted into injured mouse lung to regenerate human air exchanging units. In unperturbed lung, the SOX9+ BCs are located in the base of airway epithelium invagination, which is reminiscent of intestinal stem cells residing in gut crypt compartments. However unlike the intestinal stem cells which are constantly in active cell cycle to replenish gut epithelium in a fast turn-over mode (Clevers, 2013), the SOX9+ BCs in airway are quiescent most of the time, and could only be activated once a particular injury signal from more distal lung was received. Like its counterpart p63+/Krt5+ BCs in mouse, endogenous SOX9+ BCs might migrate towards inflamed parenchymal region and rebuild the respiratory tree by proliferation and differentiation. We and previous studies found that there are P63+ and/or KRT5+ cells enriched in the damaged alveolar region of many lung disease patients (including those with COPD, pulmonary fibrosis and bronchiectasis) (Chilosi et al., 2002; Asano et al., 2011; Smirnova et al., 2016), which could be the progeny of endogenous SOX9+ BCs in the middle of differentiation process. Interestingly there was almost no SPC+ AEC2 generated in our xeno-transplantation model, which suggested the limitation of the SOX9+ progenitor potency and also the possibility that the traditional concept of human AEC2 as the progenitor of AEC1 may not be correct in this circumstance.
The pattern that SOX9+ BCs adopt to regenerate the respiratory tree resembles the natural development process of lung in gestation, which raises an open question as whether SOX9+ BCs are the remains of previously documented SOX9+ progenitors in embryonic lung. In embryonic lung, SOX9+ embryonic progenitors are enriched in distal bud tips of respiratory tree at canalicular stage (Perl et al., 2005). Interestingly, previous report demonstrated that intravenous transplantation of human canalicular-stage embryonic lung cell mixture into NOD-SCID mice can give rise to chimeric lung (Rosen et al., 2015). Similarly, a more recent report showed mouse SOX9+ progenitors in embryonic lung can be grown in vitro as organoid and transplanted to generate mouse alveoli (Nichane et al., 2017). Altogether these work supported the concept that SOX9+ cells are lung progenitors in both embryonic and adult lung.
One important technical advance we bring out in this work is the system to selectively expand SOX9+ BCs in a feeder-free condition. Previously through bronchoscopic brushing followed by routine basal cell culture, Crystal et al., obtained P63+/KRT5+/SOX7/15/4+ basal cells but not the rare SOX9+ subpopulation (Hackett et al., 2011) . Here from as few as one single SOX9+ BC, we can expand it to 5 × 107 purely undifferentiated cells within 3–4 weeks. Therefore we can acquire a homogeneous population of regenerative cells with uniform characteristics, which is crucial for cell quality control in further clinical application.
Most importantly, we showed that SOX9+ BCs cultured under GMP guidelines can be applied clinically in order to reconstitute human lung for devastating chronic lung disease treatment. To the best of our knowledge, this is the first successful attempt to regenerate human large inner organ based on cell replacement strategy. As demonstrated in hematopoietic, skin and corneal regeneration field, autologous stem/progenitor cell transplantation strategy has been successfully applied to treat multiple devastating diseases. We show here that supplement of expandable SOX9+ BCs by autologous transplantation could repair the damaged lung in two bronchiectasis patients in both pulmonary structure and function. Generally the bronchiectasis patients without medical intervention will deteriorate over time, thus the recovery of lung function and structure after cell therapy suggested the efficacy of this strategy, and established a basis for future trials. As the SOX9+ BCs are derived from patients’ own airway, it is a recapitulation and augmentation of naturally occurring lung repair process. However after all, our pilot clinical trial is a very preliminary exploratory study so the safety and efficacy of the current strategy still need additional verification in a much larger cohort. Although we have never observed aberrant growth of SOX9+ BCs in NOD-SCID mouse model, longer time follow-up on the patients is still necessary to fully eliminate the tumorigeneic possibility. We have demonstrated the differentiation potential of SOX9+ BCs in mouse model, but the exact fate of transplanted SOX9+ BCs in human lung remains to be proven with future development of non-invasive cell tracking techniques. Furthermore, we have demonstrated that SOX9+ BCs derived from normal or diseased people can both give rise to multiple lineages of lung epithelial cells, but detailed quantitative comparisons of the regenerative capacity between normal and diseased persons would require a larger sample size investigation in future.
In conclusion, our study clearly shows the capability of SOX9+ BCs to regenerate human lung, proves the concept of chronic lung disease treatment by SOX9+ BC transplantation and provides exciting translational opportunities in near future.
Human tissue collection
Patients without or with chronic lung diseases (COPD, bronchiectasis and ILD) were diagnosed by ATS/ERS criteria. All individuals went through thorough medical examination before sampling. The bronchoscopic procedure for sampling was performed by board-certified respiratory physicians using a flexible fiber-optic bronchoscope (Olympus, Japan). Before the bronchoscopy, oropharyngeal and laryngeal anesthesia was obtained by administration of 2 mL of nebulized 4% lidocaine, followed by 1 mL of 2% topical lidocaine sprayed into the patient’s oral and nasal cavities. After the bronchoscope was advanced through the vocal cords, 2 mL of 2% lidocaine solution was instilled into the trachea and both main bronchi through the working channel of the bronchoscope. Then a disposable 2-mm brush was advanced through the working channel of the fiberoptic bronchoscope and used to collect airway epithelial cells by gently gliding the brush back and forth 1 or 2 time in random regions of trachea or 3–4 order bronchi in the right or left lobe. No obvious differences were observed between the BC clones isolated from 3rd vs. 4th order bronchi, or from different lung lobes. For bulk lung sampling, normal human lung bulk samples were collected from unaffected lung area of lung cancer patients with open chest surgery. All the human tissues were obtained following clinical SOP under patient’s consent and approved by Southwest Hospital Ethics Committee (Chongqing, China) and Shanghai East Hospital Ethics Committee (Shanghai, China).
Isolation and culture of human SOX9+ BCs
To isolate the SOX9+ BCs, 2 mm brush with samples were cut with scissors into 1 cm pieces. After removing sputum, the brush pieces were directly digested with dissociation buffer including DMEM/F12 (Gibco, USA), 2 mg/mL protease XIV (Sigma, USA), 0.01% trypsin (Gibco, USA) and 10 ng/mL DNase I (Sigma, USA). Specimens were incubated at 37°C for an hour with gentle rocking. Alternatively, human small airway were dissected from a bulk of lung tissue and digested in the same dissociation buffer at 37°C overnight. Dissociated cells were passed through 70-μm Nylon mesh (Falcon, USA) to remove aggregates and then washed twice with cold F12 medium. Cell viability was assessed by exclusion of trypan blue dye. Cell pellets were collected by centrifuge of 200 ×g and plated onto mitomycin-inactivated 3T3 feeder cells in BC culture medium for lung (BCM-L) including DMEM/F12 (Gibco, USA), 10% FBS (Hyclone, Australia), antibiotics, amphotericin and growth factor cocktail as previously described (Zuo et al., 2015). Under 7.5% CO2 culture condition, the SOX9+ BC colonies emerged 3–5 days after plating, and were digested by 0.25% trypsin-EDTA (Gibco, USA) for 3–5 min for passaging. Typically, SOX9+ BCs are passaged every 5 to 7 days and split at 1:7 ratio. To obtain single cell-derived clone, cells are digested into single cells, loaded through 40-μm Nylon mesh and seeded with extremely low density, then a single colony grown up from a single cell was picked up by clone cylinder (Sigma, USA) and high vacuum grease after its neighboring colonies were cleared by scraper to ensure the pedigree purity. For feeder-free culture of SOX9+ BCs, feeder cells were removed by differential trypsinization with 0.05% trypsin (Gibco, USA) and SOX9+ BCs were plated with high density onto dishes pre-coated with 15% cold collagen type I (Corning, USA) and 20% Matrigel (Corning, USA) for further expansion.
For labeling of cells by GFP, pLenti-CMV-EGFP plasmid was transfected into 293T cells together with lentivral packaging mix (Life Technologies, USA). Lentivirus supernatant produced by 293T was collected, filtered and cryo-preserved before use. To infect SOX9+ BCs, 0.5 mL lentivirus containing medium was directly added to 2 mL cell culture medium with 10 μg/mL polybrene and incubated for 12 h. The overall labeling efficiency of cells is above 95%. To confirm that GFP containing virus will not spread between cells after labeling, we co-cultured GFP-labeled SOX9+ BCs with mCherry-labeled (pLenti-CMV-mCherry) SOX9+ BCs for 5 days and did not observe any yellow color cells.
For immunofluorescence staining, cells were fixed by 3.7% formaldehyde, and then incubated with 0.3% Triton X-100 to improving the cell permeability for 10 min. Paraffin- or cryo-embedded tissues were sectioned and subjected to antigen retrieval in citrate buffer (pH 6.0, Sigma, USA) in microwave oven for 20 min before staining. 10% normal donkey serum (Jackson ImmunoResearch) was used to block the non-specific antigen. Primary antibodies used in this work include BC markers:KRT5 (1:200, EP1601Y, Thermo), P63 (deltaN, 1:200, 4A4, Abcam), E-cadherin (1:200, H-108, Santa cruz), SOX9 (1:200, ERP14335-78, Abcam), SOX9 (1:200, AF3075, R&D); AEC markers: AQP5 (1:1000, EPR3747, Abcam), HOPX (1:500, E-1, Santa Cruz), PDPN (1:500, FL-162, Santa Cruz), SPC (1:200, M-20, Santa Cruz), SPC (1:200, FL-197, Santa Cruz), LAMP3 (1:200, 12632-1-AP, Proteintech); bronchiolar cell markers: CC10 (1:200, T-18, Santa Cruz), acetylated-α-Tubulin (1:1000, 6-11B-1, Abcam), MUC5AC (1:500, 45M1, Thermo), FOXJ1 (1:200, 2A5, eBioscience); vasculature markers: CD31 (1:100, M-20, Santa Cruz), CD34 (1:1000, EP373Y, Abcam); myofibroblast marker: α-SMA (1:500, 1A4, DAKO), Fibronectin (1:500, F14, Abcam), others: KI67 (1:200, RM-9106, Thermo), GFP (1:200, B-2, Santa Cruz), GFP (1:200, FL, Santa Cruz), GFP (1:200, T-19, Santa Cruz), ITGB1 (1:500, ERP16895, Abcam), Human specific Lamin A+C (1:200, EPR4100, Abcam). Alexa Fluor-conjugated Donkey 488/594/647 (1:200, Life Technologies, USA) were used as secondary antibodies. For antibodies of low reactivity, Biotin-Streptavidin signal amplification system (Life Technologies, USA) was used. After counterstaining with DAPI (Roche, USA), samples were treated with 0.1% Sudan Black (Sigma, USA) for 1 min to remove autofluorescence and then mounted with VECTASHIELD® Mounting medium (Vector labs, USA). Images were visualized under fluorescence microscope (Nikon 80i and Eclipse Ti, Nikon, Japan) or fluorescence stereomicroscope (MVX10, Olympus, Japan). Confocal images were taken under Nikon A1R microscope (Nikon, Japan).
RNA-sequencing and bioinformatics
SOX9+ BCs isolated from two donors and their corresponding brush-off specimens were subjected to RNA-Seq analysis. The total RNA concentration and RIN were measured by Agilent 2100 Bioanalyzer (Agilent). For human SOX9+ BCs, 200 ng total RNA sample was purified, and the first-strand cDNA was synthesized using first strand master mix and super script II (Life Technologies). Second strand master mix (Life Technologies) was then used to synthesize the second-strand cDNA. After cDNA purification and adapter ligation, PCR amplification was performed to enrich the cDNA fragments. For brush-off samples, after RNA extraction and quality control, cDNA was prepared using the SMARTer Ultra Low RNA Kit (Clontech) for Illumina sequencing. Low Input Library Prep Kit (Clontech) was then used for library construction. The library quantity and quality was verified by Agilent 2100 Bioanalyzer and real-time quantitative PCR. Then the library is sequenced using Illumina HiSeq 4000. Clean data were acquired from raw data (fastq format) using the NGSQC Toolkit by removing low-quality reads. Clean RNA-seq reads were mapped to the reference genome (Ensembl, GRCh37) using Tophat v2.0.049 using default settings.
With genome mapping result, gene expression level was calculated with RSEM software (v1.2.12). Transcript levels were quantified as fragments per kilobase of transcript per million mapped reads (FPKM). Pearson correlation coefficient between samples was calculated by R scripts (3.2.3). Heatmap was generated using R scripts. The protein-protein interactions were retrieved from Human Protein Reference Database (HPRD, release 9) and visualized with Cytoscape (v3.3.0). SNPs were called by GATK (v3.4-0).
To arrest SOX9+ BCs in mitosis metaphase, cells of 75% confluence were treated with 1 μg/mL colchicines for 7 h and digested into single cells by 0.25% trypsin. Then the cells were incubated by 0.4% KCl at 37°C for 40 min and fixed by 10 mL fixation solution including methanol and glacial acetic acid (3:1) at room temperature for 30 min. Suspension with chromosomes was dropped and spread on slides. Samples on slides were treated by 0.0005% trypsin for 5 min and stained with 15% Giemsa (Sigma-Aldrich, USA). Banding patterns on chromosome spreads were checked for more than 15 mitotic phases and all of them are normal human cells. All cells used for clinical purpose were subjected to karyotyping in prior to transplantation.
Quantitative reverse transcription PCR
Total RNA from tissues or cells were isolated using the RNeasy mini kit with DNase digestion according to the manufacturer’s instructions (Qiagen). RNA quality was determined by SimpliNano (GE Healthcare). 1 μg total RNA was reverse-transcribed into cDNA with PrimeScript™1st Strand cDNA synthesis Kit (TaKaRa). The real-time PCR assays were performed on an ABI 7500 real-time PCR system (Applied Biosystems) according to the instructions of SYBR® Premix Ex Taq™II (Tli RNaseH Plus, Takara). qPCR reactions were set as following: 95°C for 2 min, then 40 cycles of 95°C for 10 s, and 60°C for 40 s. Melt curve stage was added after PCR amplification stage. The threshold crossing value (Ct) of each transcript was normalized to reference genes (β-Actin or GAPDH). The relative expression level of each genes was calculated using the 2−ΔΔCt method. Sequence of primer pairs for qPCR was listed in Supplementary Table.
Animal tissue histology
All animal experiments were conducted according to guidelines approved by University Association for Laboratory Animal Science. NOD-SCID mice (female or male, 6–10 weeks, The Jackson Laboratory, USA) were euthanized at proper time points and the diaphragm was carefully cut open without touching the lung. In situ fixation by injecting 3.7% formaldehyde (Sigma, USA) through trachea was performed using 29 G needle. Then the lung was dissected and fixed in 3.7% formaldehyde at 4°C overnight. For cryosection, the fixed lung was settled by 30% sucrose before embedding into the Tissue-Tek O.C.T compound (Sakura, Japan), the 5–10 μm sections were cut using a cryotome (Leica microsystem, Germany). For paraffin section, the lung was dehydrated by gradient ethanol and processed in an automatic tissue processor, then embedded into the paraffin blocks. All the samples were sliced into 5–7 μm thickness using microtome (Leica microsystem, Germany). Haematoxylin and eosin (H&E) staining was performed following standard protocol. Masson trichrome staining was performed following the manual of Trichrome Staining Kit manual.
Small animal micro-CT
Micro-CT was used to monitor mouse lung damage before transplantation. Mice were anesthetized through intraperitoneal injection with chloral hydrate and fixed with tap. Lung image was obtained using a volumetric micro-CT scanner without respiratory gating (TriumphTM, Gamma medica-ideas, Northridge, USA). Scanning was performed at 70 kV, 350 μA. The number of projections were 512 slices and total acquire time was around 4.27 min. All data were converted into digital imaging by TRIUMPH ‘X-O’ CT system software.
SOX9+ BC transplantation in mouse
Adult NOD-SCID mice (female or male, 6–10 weeks, The Jackson Laboratory, USA) maintained in SPF animal facilities were used for xeno-transplantation experiments. Mouse lung was injured by intratracheally instilling with 3 U/kg body weight bleomycin (Selleckchem, USA) eight days prior to transplantation. Mouse lung was monitored by small animal micro-CT before transplantation to verify lung damage. Then mice were anesthetized by I.P injection of 3% chloral hydrate and rested on a stand gesture. One million GFP-labeled cells were suspended in 50 μL PBS and used for transplantation of each mouse. Intratracheal aspiration was performed by injecting the cells into trachea via mouth. Three weeks after transplantation, the lung samples were collected for analysis.
Fluorescence compatible optical clearing of lung sample
Optical clearing of SOX9+ BC transplanted lung was performed following the SeeDB protocol of Meng-Tsen Ke et al., (2013) with minor modification. Briefly, a whole lobe of lung was fixed by 3.7% formaldehyde, and then transferred into 20%, 40%, 60%, 80% and 100% (w/v) fructose solution containing 0.5% α-thioglycerol. In each gradient solution lung was incubated for 12 h at RT. In the end, lung was transferred into SeeDB solution (80.2% w/w fructose) for 48 h to 72 h. The GFP fluorescence and blood vessels were directly visualized by fluorescence stereomicroscope.
Tracing intravascular transport by nanoparticles
Water soluble 5 nm gold nanoparticles (AuNPs) were synthesized as described previously (Cheng et al., 2008) with minor modifications: 0.25 mmol tetra-n-octylammonium bromide (TOAB) and 0.6 mmol dodecylamine (DDA) dissolving in 5 mL of toluene was mixed with 0.53 mmol HAuCl4 solution (30% in HCl solution). A 2 mmol cold NaBH4 aqueous solution was added into the organic phase and stirred vigorously for 2 h. The DDA-AuNPs were collected by precipitation in 40 mL of ethanol and then redispersed in 3 mL of chloroform. Next, MeO-PEG-SH (MW = 5000) and the DDA-stabilized Au nanoparticles were mixed in chloroform and stirred overnight. The organic phase was washed twice by water and then evaporated under vacuum. The residues were washed three times by water and purified by centrifugation.
To trace the intravascular transport route into lung, 10 mmol/L AuNPs were dissolved in 50 μL PBS and injected intravenously into mouse tail. To trace the aspiration route into lung, 10 mmol/L AuNPs were dissolved in 50 μL PBS and instilled intratracheally into mouse lung. One hour later, the lung was collected and then briefly fixed in 3.7% formaldehyde for 30 min on ice, and then embedded into the Tissue-Tek O.C.T compound followed by cryosections. GFP signal on tissue slide was captured by direct immunofluorescence and then the same slide was stained with LI Silver Enhancement Kit following manufacturer’s instruction (Thermo, USA). Brown color indicates the precipitation of AuNPs after reaction with silver.
Cells were washed in cold PBS and harvested by plastic scraper. Collected lung tissues were washed in cold PBS, ground and lysed by electric tissue grinder in RIPA buffer (150 mmol/L sodium chloride, 0.5% Triton-X100, 0.5% sodium deoxycholate, 5 mmol/L EDTA, 0.1% SDS, 50 mmol/L Tris-HCl, pH 7.5) with protease inhibitors cocktail (Roche, USA). Approximately 30 μg total protein from each sample was loaded. Samples were separated on a 10% SDS poly-acrylamide gel and transferred to PVDF membranes (Roche, USA) with electrophoresis blotting transfer apparatus. The membranes were blocked with 5% dehydrated milk for 1.5 h and then incubated with primary antibodies overnight. The next day, the membranes were incubated with horseradish peroxidase-conjugated secondary antibody. The specific signals were detected by ECL plus western blotting detection reagents and X-ray film system.
Flow cytometry analysis
For immunostaining, cells were fixed by 3.7% formaldehyde for 30 min and permealized by 0.2% Triton X-100 for 5 min. 0.5% donkey serum was used to block the non-specific signals at room temperature for 30 min. Then the samples were incubated sequentially with primary antibody and FITC/APC-Cy7-conjugated secondary antibody (1:400, Life technologies, USA) at room temperature for 1–2 h. BD FACS Verse (BD, USA) equipped with 488 and 647 lasers was used to detect the fluorescence signals for samples. Single cell suspensions went through 40 μm strainer before test. FSC-A and SSC-A parameters were used to exclude the debris and FSC-H, FSC-W, SSC-W parameters were used to exclude the clusters in the cell suspension. IgG control sample was used to set the bottom-line of the positive signals.
SOX9+ BC transplantation clinical trial
A prospective, single-center, non-randomized clinical study was conducted to evaluate the feasibility, safety and efficacy of SOX9+ BC transplantation in patients with bronchiectasis. The trial was approved by Southwest Hospital Ethics Committee (Chongqing, China, 2016-Research-#19,ClinicalTrials.gov: NCT02722642), conducted in compliance with Good Clinical Practice (GCP) standard and the most recent version of the Declaration of Helsinki. Two patients who had signed informed consent form were admitted to hospital twice for SOX9+ BC isolation and transplantation, respectively. Diagnosis was established based on ATS/ERS guidelines. Patient medical history, vital signs, routine laboratory tests (regular blood counts, biochemical measurements, coagulation test, liver/renal function tests, myocardiozymogram measurements), electrocardiogram, arterial blood gas, pulmonary function tests and HRCT scan were conducted based on standardized clinical SOP of hospital 1 day before and different times after SOX9+ BC transplantation. More detailed information for the clinical trial was described in Supplementary Materials.
Block randomization was used to randomize samples/mice into groups of similar sample size. No samples, animals or patients were excluded from all analysis. Statistical analysis was performed by Student’s t-tests (two-tail comparisons) or Wilcox test and significant difference was defined as P < 0.05. Values in text were presented as means with S.E.M. Microsoft Excel 2011 (Microsoft, USA) or R programming was used for data management, statistical analysis and graph generation. Statistical power analysis was used to ensure adequate sample size for detecting significant difference between samples. The variance is similar between groups that are being statistically compared. All experiments (except the clinical trial) were replicated for at least three times with consistent results in the laboratory. All experimental including the clinical trial outcomes were assessed by at least one blinded participating investigator.
This work was funded by The National Key Research and Development Program of China (2017YFA0104600), Youth 1000 Talent Plan of China to W. Zuo, Tongji University (Basic Scientific Research-Interdisciplinary Fund and 985 Grant to W. Zuo), Shanghai Pulmonary Hospital (Annual Grant to W. Zuo), National Science Fund Committee of China (81570091 and 81770073 to W. Zuo), Academic Leadership Fund of Shanghai (16XD1403100 to T. Ren), Postdoc Grant of China (2016M601651 to Y. Ma and 2016M591716 to Q. Ma) and Kiangnan Stem Cell Institute. We thank Prof. Zhongwei Li for comment on the manuscript, and thank Profs. Frank McKeon, Wa Xian and Nanshan Zhong for helpful discussion of this work, and thank Profs. Xiaoqing Zhang, Long Zhang and Huiping Li for reagents help.
COMPLIANCE WITH ETHICS GUIDELINES
Qiwang Ma, Yu Ma, Xiaotian Dai, Tao Ren, Yingjie Fu, Wenbin Liu, Yufei Han, Yingchuan Wu, Yu Cheng, Ting Zhang and Wei Zuo declare that they have no conflict of interest. All institutional and national guidelines for the care and use of laboratory animals were followed. All procedures followed were in accordance with the ethical standards of the responsible committee on human experimentation (institutional and national) and with the Helsinki Declaration of 1975, as revised in 2000 (Mannino 2002). Informed consent was obtained from all patients for being included in the study.
- Chapman HA, Li X, Alexander JP, Brumwell A, Lorizio W, Tan K, Sonnenberg A, Wei Y, Vu TH (2011) Integrin alpha6beta4 identifies an adult distal lung epithelial population with regenerative potential in mice. The Journal of clinical investigation 121:2855–2862. https://doi.org/10.1172/JCI57673 CrossRefPubMedPubMedCentralGoogle Scholar
- Cheng Y, Samia CA, Meyers JD, Panagopoulos I, Fei B, Burda C (2008) Highly efficient drug delivery with gold nanoparticle vectors for in vivo photodynamic therapy of cancer. Journal of the American Chemical Society 130:10643–10647. https://doi.org/10.1021/ja801631c CrossRefPubMedPubMedCentralGoogle Scholar
- Chilosi M, Poletti V, Murer B, Lestani M, Cancellieri A, Montagna L, Piccoli P, Cangi G, Semenzato G, Doglioni C (2002) Abnormal re-epithelialization and lung remodeling in idiopathic pulmonary fibrosis: the role of deltaN-p63. Laboratory investigation; a journal of technical methods and pathology 82:1335–1345CrossRefPubMedGoogle Scholar
- Hogan BL, Barkauskas CE, Chapman HA, Epstein JA, Jain R, Hsia CC, Niklason L, Calle E, Le A, Randell SH, Rock J, Snitow M, Krummel M, Stripp BR, Vu T, White ES, Whitsett JA, Morrisey EE (2014) Repair and regeneration of the respiratory system: complexity, plasticity, and mechanisms of lung stem cell function. Cell stem cell 15:123–138. https://doi.org/10.1016/j.stem.2014.07.012 CrossRefPubMedPubMedCentralGoogle Scholar
- Huang SX, Islam MN, O’Neill J, Hu Z, Yang YG, Chen YW, Mumau M, Green MD, Vunjak-Novakovic G, Bhattacharya J, Snoeck HW (2014) Efficient generation of lung and airway epithelial cells from human pluripotent stem cells. Nature biotechnology 32:84–91. https://doi.org/10.1038/nbt.2754 CrossRefPubMedGoogle Scholar
- King TE, Bradford WZ, Castro-Bernardini S, Fagan EA, Glaspole I, Glassberg MK, Gorina E, Hopkins PM, Kardatzke D, Lancaster L, Lederer DJ, Nathan SD, Pereira CA, Sahn SA, Sussman R, Swigris JJ, Noble PW, Group AS (2014) A phase 3 trial of pirfenidone in patients with idiopathic pulmonary fibrosis. The New England journal of medicine 370:2083–2092. https://doi.org/10.1056/nejmoa1402582 CrossRefPubMedGoogle Scholar
- Mou H, Vinarsky V, Tata PR, Brazauskas K, Choi SH, Crooke AK, Zhang B, Solomon GM, Turner B, Bihler H, Harrington J, Lapey A, Channick C, Keyes C, Freund A, Artandi S, Mense M, Rowe S, Engelhardt JF, Hsu YC, Rajagopal J (2016) Dual SMAD Signaling Inhibition Enables Long-Term Expansion of Diverse Epithelial Basal Cells. Cell stem cell 19:217–231. https://doi.org/10.1016/j.stem.2016.05.012 CrossRefPubMedPubMedCentralGoogle Scholar
- Rajagopal J, Carroll TJ, Guseh JS, Bores SA, Blank LJ, Anderson WJ, Yu J, Zhou Q, McMahon AP, Melton DA (2008) Wnt7b stimulates embryonic lung growth by coordinately increasing the replication of epithelium and mesenchyme. Development 135:1625–1634. https://doi.org/10.1242/dev.015495 CrossRefPubMedPubMedCentralGoogle Scholar
- Rockich BE, Hrycaj SM, Shih HP, Nagy MS, Ferguson MA, Kopp JL, Sander M, Wellik DM, Spence JR (2013) Sox9 plays multiple roles in the lung epithelium during branching morphogenesis. Proceedings of the National Academy of Sciences of the United States of America 110:E4456–4464. https://doi.org/10.1073/pnas.1311847110 CrossRefPubMedPubMedCentralGoogle Scholar
- Rosen C, Shezen E, Aronovich A, Klionsky YZ, Yaakov Y, Assayag M, Biton IE, Tal O, Shakhar G, Ben-Hur H, Shneider D, Vaknin Z, Sadan O, Evron S, Freud E, Shoseyov D, Wilschanski M, Berkman N, Fibbe WE, Hagin D, Hillel-Karniel C, Krentsis IM, Bachar-Lustig E, Reisner Y (2015) Preconditioning allows engraftment of mouse and human embryonic lung cells, enabling lung repair in mice. Nature medicine 21:869–879. https://doi.org/10.1038/nm.3889 CrossRefPubMedGoogle Scholar
- Tsao PN, Chen F, Izvolsky KI, Walker J, Kukuruzinska MA, Lu J, Cardoso WV (2008) Gamma-secretase activation of notch signaling regulates the balance of proximal and distal fates in progenitor cells of the developing lung. The Journal of biological chemistry 283:29532–29544. https://doi.org/10.1074/jbc.M801565200 CrossRefPubMedPubMedCentralGoogle Scholar
- Tzouvelekis A, Paspaliaris V, Koliakos G, Ntolios P, Bouros E, Oikonomou A, Zissimopoulos A, Boussios N, Dardzinski B, Gritzalis D, Antoniadis A, Froudarakis M, Kolios G, Bouros D (2013) A prospective, non-randomized, no placebo-controlled, phase Ib clinical trial to study the safety of the adipose derived stromal cells-stromal vascular fraction in idiopathic pulmonary fibrosis. Journal of translational medicine 11:171. https://doi.org/10.1186/1479-5876-11-171 CrossRefPubMedPubMedCentralGoogle Scholar
- Vaughan AE, Brumwell AN, Xi Y, Gotts JE, Brownfield DG, Treutlein B, Tan K, Tan V, Liu FC, Looney MR, Matthay MA, Rock JR, Chapman HA (2015) Lineage-negative progenitors mobilize to regenerate lung epithelium after major injury. Nature 517:621–625. https://doi.org/10.1038/nature14112 CrossRefPubMedGoogle Scholar
- Wang X, Yamamoto Y, Wilson LH, Zhang T, Howitt BE, Farrow MA, Kern F, Ning G, Hong Y, Khor CC, Chevalier B, Bertrand D, Wu L, Nagarajan N, Sylvester FA, Hyams JS, Devers T, Bronson R, Lacy DB, Ho KY, Crum CP, McKeon F, Xian W (2015) Cloning and variation of ground state intestinal stem cells. Nature 522:173–178. https://doi.org/10.1038/nature14484 CrossRefPubMedPubMedCentralGoogle Scholar
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