Induced pluripotent stem cells from GMP-grade hematopoietic progenitor cells and mononuclear myeloid cells
© Ohmine et al.; licensee BioMed Central Ltd. 2011
Received: 21 July 2011
Accepted: 16 November 2011
Published: 16 November 2011
The induced pluripotent stem cell (iPSC) technology allows generation of patient-specific pluripotent stem cells, thereby providing a novel cell-therapy platform for severe degenerative diseases. One of the key issues for clinical-grade iPSC derivation is the accessibility of donor cells used for reprogramming.
We examined the feasibility of reprogramming mobilized GMP-grade hematopoietic progenitor cells (HPCs) and peripheral blood mononuclear cells (PBMCs) and tested the pluripotency of derived iPS clones.
Ectopic expression of OCT4, SOX2, KLF4, and c-MYC in HPCs and PBMCs resulted in rapid iPSC derivation. Long-term time-lapse imaging revealed efficient iPSC growth under serum- and feeder-free conditions with frequent mitotic events. HPC- and PBMC-derived iPS cells expressed pluripotency-associated markers, including SSEA-4, TRA-1-60, and NANOG. The global gene-expression profiles demonstrated the induction of endogenous pluripotent genes, such as LIN28, TERT, DPPA4, and PODXL, in derived iPSCs. iPSC clones from blood and other cell sources showed similar ultrastructural morphologies and genome-wide gene-expression profiles. On spontaneous and guided differentiation, HPC- and PBMC-derived iPSCs were differentiated into cells of three germ layers, including insulin-producing cells through endodermal lineage, verifying the pluripotency of the blood-derived iPSC clones.
Because the use of blood cells allows minimally invasive tissue procurement under GMP conditions and rapid cellular reprogramming, mobilized HPCs and unmobilized PBMCs would be ideal somatic cell sources for clinical-grade iPSC derivation, especially from diabetes patients complicated by slow-healing wounds.
Because embryonic stem (ES) cells can self-renew indefinitely and differentiate into any cell present in the adult organism, ES cells provide a unique platform for regenerative medicine approaches. In early 2009, the US Food and Drug Administration (FDA) approved the first clinical trial using ES cells in patients with spinal cord injuries. Although the FDA temporarily placed the trial on hold because of concerns over the risk of ES-derived cyst formation, the clinical hold was lifted, and the first patient for ES cell treatment was enrolled by Geron in late 2010 . The use of ES-derived, terminally differentiated retinal pigment epithelium cells for Stargardt macular dystrophy and dry age-related macular degeneration was also approved by the FDA, and Advanced Cell Technology is currently enrolling patients . Despite these advances in clinical applications, the use of ES cells is associated with ethical issues and immunologic mismatch, which could affect their widespread use in the clinic.
The induced pluripotent stem cell (iPSC) technology allows generation of autologous pluripotent stem cells without using an embryonic cell source. Expression of the transcription factors OCT3/4, SOX2, KLF4, and c-MYC [3–7] or OCT-3/4, SOX2, NANOG, and LIN28  in somatic cells results in iPSCs, which have phenotypes very similar to those of ES cells, including the morphology, self-renewal, and pluripotent potentials, and expression of pluripotency-associated factors, including SSEA-4 and TRA-1-60. Global gene-expression analysis of human iPSCs has also revealed patterns similar to those of human ES cells, with notable upregulation of pluripotency-associated genes such as OCT4, SOX2, NANOG, TERT, and DPPA4 [3–5, 8]. Similar to ES cells, iPSCs can be differentiated into various cell types, such as insulin-producing cells [9–11], neurons , cardiomyocytes [13–15], and cells of hematopoietic lineages . Various types of somatic cells have been successfully reprogrammed, including fibroblasts, stomach and liver cell cultures , human keratinocytes (HKs) [17, 18], frozen human monocytes , cord blood cells [20–22], and blood cells [23, 24], including mature B [25–28] and T lymphocytes [29–32]. For clinical applications, it would be ideal if iPSCs could be generated from somatic cells through a minimally invasive tissue-procurement procedure under GMP-compliant process. In this regard, blood cells are one of the most promising cell sources for clinical-grade iPSC derivation.
Here we examined the feasibility of iPSC derivation from GMP-grade mobilized hematopoietic progenitor cells (HPCs) and unmobilized peripheral blood mononuclear cells (PBMCs), and characterized derived iPSCs for global gene-expression profiles and pluripotency.
Materials and methods
All studies were approved by the Institutional Review Board and Institutional Animal Care and Use Committee.
GMP-grade HPCs were originally harvested from patients for stem cell therapy. Specifically, HPCs were harvested after mobilization by injection with granulocyte colony-stimulating factor for 5 days in the Human Cellular Therapy Laboratory at the Mayo Clinic. Those cell products are routinely discarded as clinical wastes when patients have died before the initiation of stem cell therapy. We received de-identified clinical-waste HPCs from the Human Cellular Therapy Laboratory for iPSC derivation. The use of clinical-waste HPCs for iPSC generation was approved by the Institutional Review Board, including the Biospecimens Subcommittee. For mononuclear myeloid cell derivation, 10 ml of whole blood was purchased and used to isolate PBMCs, as reported previously [33, 34].
Lentiviral vector production
Pluripotency-associated factor-expressing lentiviral vectors, pSIN-OCT4, pSIN-SOX2, pSIN-KLF4, and pSIN-cMYC were described previously . These vectors were produced by transient transfection of 293T cells. Vector titers were determined with immunostaining .
HPCs and PBMCs were cultured overnight in StemSpan H3000 serum-free medium (StemCell Technologies, Vancouver, Canada), which contains only human-derived or recombinant human proteins, supplemented with StemSpan CC100 cytokine cocktail (StemCell Technologies). Cells (105 cells/500 μl of medium in each well) in uncoated wells of a 24-well plate were then transduced with four stemness factor-expressing lentiviral vectors overnight. One third of the culture supernatants were carefully removed and replaced daily with H3000 growth medium supplemented with CC100 cytokine cocktail. Three days after vector infection, cells in a well of a 24-well plate were transferred to a Matrigel (BD Biosciences, Bedford, MA)-coated well of a 6-well plate. Starting 5 days after vector infection, cells were maintained in HEScGRO medium (100 ml; Millipore, Billerica, MA) supplemented with mTeSR-1 maintenance media (25 ml; StemCell Technologies) . 7 to 10 days after vector infection, the reprogrammed cells began to form colonies with iPS morphology. At 2 to 3 weeks after vector infection, cultures were treated with Cell Dissociation Buffer (Invitrogen, Grand Island, NY) for 5 to 10 minutes to help lift clones, and individual iPSC-like clones were carefully picked up with a P200 pipette, and placed into Matrigel-coated wells in a 96-well plate. To prevent spontaneous differentiation, the iPSC culture medium was replaced daily, and differentiated cells in the cultures were manually removed with a pipette tip. As the clones grew, cultures were expanded into larger culture plates for further characterization. Clones were preserved by using Xeno-FREEze Human Embryonic Stem Cell Freezing Medium (Millipore). A verified iPSC clone, HCF1, from primary human fibroblast (HCF) cells, was described previously . Primary human keratinocytes and keratinocyte-derived iPSC clones were also used as controls .
Immunostaining and alkaline phosphatase staining
For immunostaining of iPSC, cells were fixed for 20 minutes at room temperature in 4% paraformaldehyde solution in PBS, washed several times in PBS, and blocked for 30 minutes in PBS with 5% fetal bovine serum. Cells were then stained with primary antibodies overnight at 4°C, rinsed with PBS, and incubated with secondary antibodies for 1 hour at RT. For immunostaining of differentiated cells, cells at different stages of differentiation were fixed and stained with primary and secondary antibodies. Primary antibodies used for characterization of iPSC and iPSC-derived cells were SSEA-4 and TRA-1-60 (Millipore, #SCR001), OCT4 (Cell Signaling Technology, #2750, Danvers, MA), NANOG (Abcam, #ab21624, Cambridge, MA), mouse anti-SOX17 (R&D Systems, #MAB1924, Minneapolis, MN), rabbit anti-HNF3 beta/FOXA2 (Millipore, #07-633), rabbit anti-PDX1 (Santa Cruz Biotechnology, #sc-25403, Santa Cruz, CA) and mouse anti-insulin (Sigma, #I2018, St. Louis, MO). Texas Red-conjugated donkey-anti-rabbit IgG (Jackson ImmunoResearch Laboratories, #711-075-152, West Grove, PA), Texas Red-conjugated donkey-anti-mouse IgG (Jackson ImmunoResearch Laboratories, #715-075-151), FITC-conjugated donkey-anti-rabbit IgG (Jackson ImmunoResearch Laboratories, #711-095-152), and FITC-conjugated donkey-anti-mouse IgG (Jackson ImmunoResearch Laboratories, #715-095-151) were used as secondary antibodies. DAPI was used for counterstaining. Stained cells were analyzed by using a confocal laser-scanning microscope (Zeiss, LSM 510 confocal scanning laser system).
For spontaneous differentiation, iPSC clones were dissociated by using collagenase IV for 30 minutes and plated on low-adhesion plates in basal HEScGRO medium without bFGF. Embryoid bodies (EBs) were cultured as a suspension for 7 to 10 days and adherent in DMEM with 20% FBS for additional 7 to 10 days. For immunofluorescence analysis, cells were fixed with 4% PFA for 20 minutes at RT. Immunostaining was performed as described earlier. Primary antibodies against FOXA2 for endoderm, beta-III tubulin (Abcam, #41489) for ectoderm, and CD31 (Santa Cruz Biotechnology, #SC1506) for mesoderm were used, whereas Texas Red-conjugated donkey anti-rabbit IgG (Jackson ImmunoResearch Laboratories, #711-075-152), and FITC-conjugated donkey anti-chicken IgG (Jackson ImmunoResearch Laboratories, #703-095-155) served as secondary antibodies.
In vivo differentiation of derived iPS cells
SCID-beige mice were anesthetized, and the kidney was externalized for iPS transplantation under the kidney capsule. A small incision was made in the kidney capsule, and a blunt needle used to create a pocket under the kidney capsule. After iPSC injection into the pocket, the kidney was placed back into the abdomen, and the incision closed with a Vicryl suture. Mice were maintained for 4 weeks and killed for harvesting normal and iPS-transplanted kidneys. OTC-embedded frozen tissues were cryo-sectioned for H&E staining.
Differentiation of derived iPS cells into insulin-producing cells iPSCs were differentiated into insulin-producing cells, as reported previously with minor modifications . At the first step of differentiation, human iPSC clones were treated with 25 ng/ml Wnt3a (R&D Systems) and 100 ng/ml activin A (Peprotech, Rocky Hill, NJ) in advanced RPMI (Invitrogen) with Pen/Strep for 1 day, followed by treatment with 100 ng/ml activin A in advanced RPMI supplemented with 0.2% fetal calf serum (FBS) (Invitrogen) for 2 days. At step two, cells were cultured in high-glucose DMEM (Invitrogen), supplemented with 20% (vol/vol) advanced RPMI medium containing 50 ng/ml FGF10 (R&D systems), 0.25 μmol/L KAAD-cyclopamine (CYC), and 2% FBS for 2 days. Cells were then treated with 50 ng/ml FGF10, 0.25 μmol/L CYC, and 2 μmol/L all-trans retinoic acid (RA) (Sigma) in high-glucose DMEM (Invitrogen) supplemented with 20% advanced RPMI, Pen/Strep, 1 × B27 supplement (Invitrogen) for 4 days at step three. Cells were then cultured in the presence of 50 ng/mL FGF10, 300 nmol/L ILV (Axxora, San Diego, CA), and 55 nmol/L GLP-1 (Sigma) in DMEM (high glucose) supplemented with 20% advanced RPMI and 1 × B27 for 4 days at step four. In step five, differentiation medium included 10 μmol/L DAPT (Sigma) and 55 nmol/L GLP-1 in DMEM (high glucose) with 20% advanced RPMI and 1 × B27, and the culture lasted for 6 days.
Finally, in step six, cells were cultured in the presence of 50 ng/ml hepatocyte growth factor (HGF) (R&D systems), 50 ng/ml insulin-like growth factor 1 (IGF-1) (R&D Systems), and 55 nmol/L GLP-1 in CMRL-1066 medium (Invitrogen) with 1 × B27 for 8 days. All differentiation experiments were performed in triplicate, and repeated at least twice.
Total RNA was isolated by using TRIzol (Invitrogen) and further purified by using RNeasy Plus spin columns (QIAGEN, Valencia, CA). Turbo DNA-free DNase (Ambion, Austin, TX) was used to digest all genomic DNA that could lead to false-positive gene-expression results. The RNA quantity and purity was measured with a Nanodrop spectrophotometer (Thermo Scientific, Wilmington, DE), and the RNA integrity was determined by using the Agilent 2100 Bioanalyzer (Agilent Technologies, Santa Clara, CA). Microarray analysis was performed by using the Affymetrix HG-U133 Plus2 GeneChip Array platform (Affymetrix, Santa Clara, CA). Data were preprocessed by using standard in-house MicroArray Pre-Processing workflow, and hierarchical clustering was performed by Pearson Dissimilarity. To compare the transcriptome of blood-derived iPSCs, the data set of epidermal keratinocytes (HK, SW3, SW4, and SW8), two keratinocyte-derived iPSC clones (SW3 b and SW4 N1) and human fibroblast (FB)-derived iPSC clone HCF1  were used. A t test was performed to analyze the significance of the changes (P < 0.05) in the normalized gene-expression levels between HK and iPSC clones, or between blood-derived iPSC clones and HK- and FB-derived iPSC clones. Heatmap Builder software (kindly provided by Dr. Euan Ashley, Stanford School of Medicine) was used to generate the heatmap for the transcriptome data set. The registered GEO transcriptome database (GSM551202, human ES H9 cells; GSM452255, freshly isolated PBMC; GSM178554, mobilized HPCs) was used to analyze the similarities between blood-derived iPSCs and human ES cells or non-reprogrammed PBMCs and HPCs. Microarray data have been deposited in the NCBI Gene Expression Omnibus (GEO) and are accessible through GEO Series accession number GSE33536 (http://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?acc=GSE33536).
Results and discussion
Cellular reprogramming of HPCs and PBMCs into iPSCs
Ultrastructural studies of blood-derived iPS cells
Genome-wide transcriptome analysis of blood-derived iPS clones
Pluripotency of blood-derived iPS clones verified through in vitro differentiation
In vivo multilineage differentiation of blood-derived iPSCs
To assess the multilineage differentiation capacity of iPSCs in vivo, blood-derived iPSCs were transplanted under the kidney capsule of SCID-beige mice. After transplantation of 1 million cells, iPSCs formed cystic tumors within 4 weeks (Figure 3b). On gross inspection, iPSC-derived tumors demonstrated a complex cellular architecture with prominent vascularization and nonvascularized solid tissues. Histologic analysis revealed iPSC differentiation into endoderm lineages composed of glandular-like tissue, mesoderm lineages indicated by muscle-like tissue, and ectoderm lineages denoted by neural rosette-like structures (Figure 5b), which verified the multilineage differentiation capability of blood-derived iPSCs.
Generation of insulin-producing cells from iPSCs through guided differentiation
Next we examined the pancreatic differentiation potentials of blood-derived iPSCs. We used our guided iPSC differentiation protocol with indolactam V (ILV) and GLP-1 , with minor modifications in medium compositions, which are described in Materials and Methods. Blood-derived iPSC clones were first stimulated with activin A and Wnt3a to form definitive endoderm cells. Immunostaining revealed the efficient induction of definitive endoderm markers SOX17 and FOXA2 in iPSC-derived cells at day 5 of differentiation (Figure 3c). Derived definitive endoderm cells were further differentiated in DMEM/advanced RPMI medium containing FGF10, CYC, and 2% FBS (vol/vol) for 2 days, and maintained in high-glucose DMEM/advanced RPMI medium supplemented with FGF10, CYC, RA, and 1 × B27 for an additional 4 days. Cells were then cultured in the presence of FGF10, ILV, GLP-1, and 1 × B27 in DMEM/advanced RPMI medium for 4 days. After this step, derived cells expressed pancreatic endoderm markers, PDX1 and NKX6.1 (Figure 5d). Further differentiation of iPSC-derived pancreatic endoderm cells was performed in DMEM/advanced RPMI medium supplemented with DAPT, GLP-1, and 1x B27 for 6 days, followed by the final maturation step in the CMRL-1066 medium containing HGF, IGF-1, GLP-1, and 1 × B27 for an additional 8 days. Insulin-positive iPSC progeny were sporadically detected (Figure 5d). High levels of intracellular C-peptide (230~320 pmol/L), a byproduct of proinsulin processing during insulin secretion, were also detected in the final differentiation-stage iPSC progeny with C-peptide ELISA (data not shown). Our results demonstrate successful differentiation of blood-derived iPSCs into insulin-expressing cells in vitro.
The iPSC technology opened the exciting possibility of generating patient-specific pluripotent stem cells without using an embryonic source, which could pave the way for personalized pluripotent stem cell therapy approaches. However, because of the complexity of the iPSC technology, which typically involves ex vivo gene delivery and pluripotent stem cell manipulation, multiple issues must be addressed before autologous iPSCs can contribute to novel individualized cell therapy. One of the major issues is to develop a GMP-compliant process for clinical-grade iPSC generation. For this end, we need simple, robust, and time-effective strategies for both iPSC derivation and differentiation. Currently, skin biopsy samples are typically used for iPSC derivation. However, it takes at least several days (often weeks) to process and expand skin cells. Here, we demonstrate the feasibility of iPSC derivation from GMP-grade mobilized HPCs and unmobilized PBMCs. Although our current HPC/PBMC iPSC derivation efficiencies (two to five clones per 105 transduced cells) were similar to those of previous reports [27, 29, 31, 32], generation of iPSCs from GMP-grade, blood-derived cells represents an important step toward clinical applications of iPSCs and iPSC progeny cells. The use of HPCs and PBMCs enabled time-effective iPSC derivation, as the cells did not require long-term expansion before reprogramming. Moreover, apart from minor differences in global gene-expression profiles (Figure 4), blood-derived iPSCs were basically indistinguishable from iPSCs from other cell sources. Considering that many institutes/hospitals already have an FDA-approved GMP facility for autologous HPC processing, HPCs and PBMCs would be ideal somatic cell sources for clinical-grade iPSC derivation.
We and others have reprogrammed blood cells through genome-integrating viral vectors [37, 38]. In our lentiviral vectors, the transgenes are driven by a retroviral promoter. Because retroviral promoter is strongly suppressed in pluripotent stem cells, we speculate that the expression of transgene-derived pluripotency factors is silenced in the blood-derived iPSCs. Nevertheless, the use of integrating vectors is associated with the risk of insertional mutagenesis and sustained/reactivated expression of reprogramming factors, including a protooncogene c-MYC. Indeed, stable c-Myc vector integration in iPSCs has been linked to increased tumorigenicity in vivo . Reprogramming blood cells through non-integrating vectors or introduction of reprogramming proteins, RNAs, or miRNAs [32, 40–45] would avoid/minimize these safety concerns. We are currently testing these non-integrating reprogramming strategies for patient-specific iPSC derivation.
Although islet transplantation has shown some promising results for type 1 diabetes therapy, the shortage of matched islet replacement tissues has prevented the widespread use of this therapy in the clinic. One possible solution to overcome this shortage is to regenerate transplantable insulin-secreting cells from patient-derived iPSCs . We previously reported that ILV and GLP-1 facilitate differentiation of iPSCs into insulin-producing cells through a guided differentiation protocol . Here we demonstrate the feasibility of generating insulin-producing cells from blood-derived iPSCs. To our knowledge, this is the first report showing the generation of insulin-producing islet-like cells from blood-derived iPSCs. In contrast to skin biopsies, which involve an invasive procedure, the use of blood cells allows minimally invasive tissue procurement for iPSC derivation. Because diabetes patients often experience poor wound healing, the minimally invasive iPSC derivation from blood cell sources would be particularly advantageous for the generation of clinical-grade iPSCs from diabetes patients.
Because the use of blood cells allows minimally invasive tissue procurement under GMP conditions and rapid cellular reprogramming, mobilized HPCs and unmobilized PBMCs would be ideal somatic cell sources for clinical-grade iPSC derivation, especially from diabetes patients complicated by a slow-healing wound.
fetal bovine serum
Food and Drug Administration
human cardiac fibroblast
hepatocyte growth factor
hematopoietic progenitor cells
insulin-like growth factor 1
induced pluripotent stem cell
peripheral blood mononuclear cells
We thank Ms. Ying Li and Mr. Christopher P. Kolbert (Mayo Advanced Genomics Technology Center) and Mr. Scott I. Gamb (Mayo Electron Microscopy Core Facility) for excellent technical support for transcriptome analysis and electron microscopy. This work was supported by Mayo Foundation, Eisenberg Stem Cell Trust, Minnesota Partnership Grant, Marriott Individualized Medicine Award, Bernard and Edith Waterman Pilot Grants (to YI), Marriott Specialized Workforce Development Award in Individualized Medicine (TT), and NIH Grant DK 085516 (YK).
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