This work was supported by grants funded by the British Heart Foundation (BHF), Dinosaur Trust, McAlpine Foundation, Fondation Leducq, Fight for Sight, the Cambridge Biomedical Research Centre, National Institute of Health Research including (i) the BHF Oxbridge Centre of Regenerative Medicine [RM/13/3/30159], (ii) the BHF Cambridge Centre of Research Excellence, (iii) Addenbrooke's Hospital, Cambridge University Hospitals NHS Foundation Trust and (iv) Papworth Hospital NHS Foundation Trust, and supported the Cambridge NIHR BRC Cell Phenotyping Hub. MLO is funded by a BHF Intermediate Fellowship. FNK is funded by a BHF PhD Studentship.

A schematic of the BOEC generation protocol is shown in Figure 1.
1. Blood Collection and Density Gradient Centrifugation
<ol>
	<li>For each donor, add 3 ml of sodium citrate to each of two 50 ml conical centrifuge tubes. Collect 60 ml of blood by venipuncture and add 30 ml to each tube. Invert gently 2-3 times to mix. Use as little as 40 ml of blood in the protocol, with citrate volumes adjusted accordingly. 
	NOTE: It is essential that blood samples are processed within 2 hr of collection. Delayed processing of blood results in a marked reduction in outgrowth colony yield.</li>
	<li>Prepare new conical tubes containing density gradient centrifugation medium by first inverting the bottle several times to mix. In a sterile hood, add 15 ml of density gradient centrifugation medium per 50 ml conical tube (1 tube for every 10 ml of blood, 6 tubes per donor).</li>
	<li>Dilute blood 1:1 with Dulbecco&#39;s Phosphate-Buffered Saline (DPBS). Tilt the tube containing the density gradient centrifugation medium to an angle of 20&#176; with the work surface. Using a pipette aid and a 25 ml serological pipette, slowly layer 21 ml of diluted blood on top of the medium by gradually adding blood down the wall of the tilted tube. 
	NOTE: Doing so will minimize mixing of the blood with the density gradient layer and will produce a tighter buffy coat, as well as an enhanced yield.</li>
	<li>Centrifuge samples at 400 x g for 35 min at RT with the accelerator and the brake off.</li>
	<li>During this centrifugation period, begin the collagen coating detailed in steps 2.1 - 2.4. Ensure these steps have been completed before proceeding to step 3.1.</li>
</ol>
2. Collagen Coating of T-75 Flask and Preparation of Culture Medium
NOTE: Carry out the following steps in a cell culture hood.
<ol>
	<li>Prepare a 50 &#956;g/ml collagen solution by diluting stock Type I collagen in 10 ml of 0.02M acetic acid. Example: for collagen stock at a concentration of 4.05 mg/ml, add 123.5 &#956;L of collagen to 10 ml of 0.02 M acetic acid. Sterile filter collagen suspension prior to use.</li>
	<li>Using a serological pipette, add 7.5 ml of collagen solution to a T-75 cell culture flask. This volume gives 5 &#956;g collagen/cm2 (or 375 &#956;g/flask). Coat flask for 1 hr at RT.</li>
	<li>Prepare the endothelial growth medium used for BOEC generation by supplementing endothelial basal medium with the growth factor supplements provided by the manufacturer. Add all supplements, but do not add serum. To prepare 15 ml of BOEC generation medium, add 2.5 ml of defined fetal bovine serum (FBS) to 12.5 ml of endothelial growth medium containing the growth factor supplements.</li>
	<li>Proceed with the steps outlined in Section 3. After the 1 hr coating period, aspirate the collagen solution and wash away residual acetic acid by pipetting in 10 ml DPBS. Aspirate off the DPBS and repeat this wash step once more. If the cell suspension obtained during step 3.3 is not ready for plating at this time, add 5mL of BOEC generation medium to the flask to keep the collagen coating from drying-out.</li>
</ol>
3. Collection and Plating of PBMNCs
<ol>
	<li>Following the density gradient centrifugation outlined in step 1.4, carefully collect the buffy coat layer using a sterile plastic transfer pipette. Collection of the buffy coat should yield approximately 20 ml of cell suspension and plasma from each tube. Avoid transferring the density gradient medium.</li>
	<li>Dilute the mononuclear cell suspension 1:1 in DPBS and invert to mix. Centrifuge at RT for 20 min at 300 x g with brake and accelerator at maximum.</li>
	<li>Following centrifugation, aspirate the supernatant and resuspend cells by adding 1 ml of BOEC generation medium to each pellet and pipetting up and down repeatedly. Pool cell suspensions and top up total volume to 10 ml with the remaining medium.</li>
	<li>To get an estimation of total cell number, sample 10 &#956;l of cell suspension and dilute 50x with 490 &#956;l of Turk&#39;s solution, which will lyse red blood cells. Count a 10 &#956;l sample of the diluted cell suspension using a haemocytometer. 
	NOTE: 60mL of blood should yield approximately 100-150 x 106 white blood cells for plating.</li>
	<li>Plate entire cell suspension into a single, collagen-coated T-75 flask, top-up medium volume to 15mL/flask and culture at 37 &#176;C in a humidified atmosphere containing 5% CO2. Cells plated at this time represent passage 0. 
	NOTE: It is possible to freeze the isolated PBMNCs prior to BOEC isolation in order to derive the BOECs at a later time or in order to transport the PBMNCs to a different laboratory where the BOECs can be generated. However, it is important to note that freezing PBMNCs could reduce the efficiency of BOEC isolation. See section 8 below for method.</li>
</ol>
4. Long-term Cell Culture
<ol>
	<li>Change medium every 2 days by adding 15 ml of fresh BOEC generation medium (5:1 mixture of endothelial cell growth medium and defined FBS). For weekends, medium changes can be delayed to every 3 days. 
	NOTE: Outgrowth colonies should appear between 7 and 14 days of culture.</li>
	<li>Monitor the BOEC culture flask on days 7-14 for the appearance of outgrowth colonies. Identify colonies as circular groups of cells exhibiting a classic endothelial cobblestone morphology.</li>
	<li>Once a colony or multiple colonies are identified in the flask, continue with medium changes and allow colonies to grow to approximately 1000 to 2000 cells per colony before passaging. Determine the cell number per colony through a rough visual estimate. 
	NOTE: As a guide, it is customary to passage initial outgrowth colonies one week after the identification of the first outgrowth colony.</li>
	<li>Passage cells by rinsing flasks twice with 10 ml of DPBS. Add 5 ml of 1X trypsin-EDTA and incubate in a 37 &#176;C incubator for 5 min. After 5 min, neutralize trypsin with 10 ml of medium (containing FBS) and bring cells into suspension with repeated pipetting.</li>
	<li>Centrifuge suspension at 300 x g for 5 min, resuspend in 15 ml of fresh BOEC generation medium and plate entire cell suspension into a new T-75 flask (representing passage 1, P1). No collagen coating is required.</li>
	<li>Continue medium changes as described above until cells are confluent (roughly 3-5 x 106 cells per flask). Once confluent, passage cells as described in step 4.3. 
	NOTE: From passage 2 onwards, cells no longer require BOEC generation medium and can be cultured in endothelial cell growth medium and 10% standard heat-inactivated FBS. Collagen coating can be used as an optional step going forward, as there is evidence to suggest that the presence of collagen can enhance BOEC proliferation rates.</li>
	<li>For continued passaging, plate no fewer than 750,000 cells per T-75 flask as low cell densities can cause the BOECs to stop proliferating.</li>
</ol>
5. Freezing and Thawing BOEC Cultures
<ol>
	<li>Trypsinize cells as described in section 4.3 and centrifuge at 300 x g for 5 min. Aspirate the supernatant and resuspend in 10 ml of medium. This does not require endothelial cell growth medium; DMEM with 10% standard FBS will be sufficient. Collect a 10 &#956;l sample of the cell suspension to perform a manual cell count using a haemocytometer.</li>
	<li>Centrifuge again and resuspend at 2x106 cells/ml in ice-cold cryopreservation medium (40% DMEM with 50% FBS and 10% DMSO). Add 0.5 ml (106 cells) to each vial, place vials in an ice cold isopropanol cryopreservation vessel and place in a -80 &#176;C freezer for at least 2 hr before transferring to liquid nitrogen. Do not leave cells at -80 &#176;C for more than 24 hr.</li>
	<li>To thaw cells, add 10 ml of pre-warmed medium to a 15 ml conical centrifuge tube. 
	NOTE: When thawing out passage 1 cells, thaw into endothelial cell growth medium supplemented with 20% defined FBS for the first 2 days after thawing. This leads to a more stable cell isolation going forward.</li>
	<li>Remove cells from liquid nitrogen and thaw in a 37 &#176;C water bath with gentle agitation until only a small ice crystal is left in the vial. Add the contents of the vial drop-wise to the conical centrifuge tube and spin down at 300 x g for 5 min.</li>
	<li>Aspirate supernatant and resuspend cell pellet in 10 ml EGM-2MV+10%FBS. Add to T-75 flask and top up medium to 15 ml.</li>
</ol>
6. Characterization of BOECs by Flow Cytometry
<ol>
	<li>Once the BOEC colonies described in Section 4 have been allowed to expand, trypsinize cells as described in section 4.4 and resuspend at a concentration of 106 cells per ml in staining buffer (DPBS with 2% FBS and 2 mM EDTA).</li>
	<li>Combine 105 cells with fluorochrome-conjugated antibodies directed against CD45, CD14, CD34, CD31 (use all at 1:20 dilution) or VEGFR2 (dilute 1:10) (see Table 1 for full details). Incubate for 30 min at 4 &#176;C in the dark.</li>
	<li>Wash cells with 1 ml staining buffer and centrifuge at 300 x g for 5 min. Aspirate supernatant and resuspend in 400 &#956;l staining buffer for analysis. Keep cells at 4 &#176;C and protected from light prior to analysis.</li>
	<li>Perform cytometric analysis on a cytometer equipped to detect the fluorescently conjugated antibodies used in the assay.</li>
	<li>Use an unstained BOEC sample to identify the cell population on the cytometer by adjusting forward and side scatter voltages, as well as the voltages for the FITC and APC channels.</li>
	<li>Determine gating thresholds using isotype stained cells for each fluorochrome. Assess positivity for each cell surface marker based on the presence of a peak shift in fluorescence intensity versus isotype control for the fluorochrome being analysed.</li>
</ol>

7. Characterization of BOECs by Immunofluorescent Microscopy
<ol>
	<li>Plate BOECs in a 24-well, flat-bottom tissue culture plate without coverslips at a density of 5 x 104 cells in 500 &#956;l of endothelial cell growth medium + 10% heat-inactivated FBS per well and leave to adhere and grow at 37 &#176;C, 5% CO2 until cells cover at least 70-80% of the surface area of each well (estimate confluency by visual inspection under a light microsope).</li>
	<li>Wash cells in each well for 5 min with 1 ml of DPBS.</li>
	<li>Fix cells O/N&#160;at 4 &#176;C with 500 &#181;l of 4% paraformaldehyde solution in DPBS.</li>
	<li>Wash cells for 3 x 5 min with 1 ml of DPBS per well. Add and remove the DPBS using a pipette and an aspirator, respectively.</li>
	<li>Permeabilize cells for 3 x 10 min with 0.2% polysorbate 20 in DPBS.</li>
	<li>Incubate cells for 1 hr at RT in blocking buffer containing 10% FBS in DPBS.</li>
	<li>Stain cells at 4 &#176;C O/N in 300 &#181;l of antibody dilution buffer (0.1% bovine serum albumin in DPBS) containing primary antibodies directed against CD34 (10 &#181;g/ml), CD144 (1:300) or vWF (1:250). See Table 1 for full details.</li>
	<li>Wash off unbound primary antibodies for 5 x 10 min with DPBS.</li>
	<li>Incubate cells for 1 hr at RT&#160;with the appropriate fluorescently-labelled secondary antibody, as detailed in Table 1 (all at 1:200).</li>
	<li>Wash off unbound secondary antibodies for 5 x 10 min with DPBS.</li>
	<li>Incubate cells with 1 &#181;g/ml 4&#39;,6-diamidino-2-phenylindole (DAPI) in DPBS for 10 min at RT.</li>
	<li>Wash cells with DPBS for a further 3 x 5 min.</li>
	<li>Image cells at 100x magnification using an inverted microscope equipped with an external light source for fluorescence excitation, and capture images using an attached digital camera for subsequent analysis offline.</li>
</ol>
8. Freezing and Thawing PBMNCs
<ol>
	<li>At the end of stage 3.2, following centrifugation, aspirate the medium and manually disrupt the cell pellet with repeated pipetting up and down using a P1000 pipette tip. Add 1 ml of freezing medium, 90% serum and 10% DMSO, making sure to mix gently to produce a cell suspension. Transfer the cell suspension to a cryovial and freeze and thaw as described in Section 5.</li>
</ol>

<ol>
	<li>Yancopoulos, G. D., Klagsbrun, M., Folkman, J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Vasculogenesis,+angiogenesis,+and+growth+factors:+ephrins+enter+the+fray+at+the+border.">Vasculogenesis, angiogenesis, and growth factors: ephrins enter the fray at the border.</a> Cell. 93, 661-664 (1998).</li><li>Flamme, I., Fr&#246;lich, T., Risau, W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Molecular+mechanisms+of+vasculogenesis+and+embryonic+angiogenesis.">Molecular mechanisms of vasculogenesis and embryonic angiogenesis.</a> J Cell Physiol. 173, 206-210 (1997).</li><li>Asahara, T., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Isolation+of+putative+progenitor+endothelial+cells+for+angiogenesis.">Isolation of putative progenitor endothelial cells for angiogenesis.</a> Science. 275, 964-967 (1997).</li><li>Shi, Q., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Evidence+for+circulating+bone+marrow-derived+endothelial+cells.">Evidence for circulating bone marrow-derived endothelial cells.</a> Blood. 92, 362-367 (1998).</li><li>Ormiston, M. L., Deng, Y., Stewart, D. J., Courtman, D. W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Innate+immunity+in+the+therapeutic+actions+of+endothelial+progenitor+cells+in+pulmonary+hypertension.">Innate immunity in the therapeutic actions of endothelial progenitor cells in pulmonary hypertension.</a> Am J Respir Cell Mol Biol. 43, 546-554 (2010).</li><li>Hur, J., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Characterization+of+two+types+of+endothelial+progenitor+cells+and+their+different+contributions+to+neovasculogenesis.">Characterization of two types of endothelial progenitor cells and their different contributions to neovasculogenesis.</a> Arterioscler Thromb Vasc Biol. 24, 288-293 (2004).</li><li>Lin, Y., Weisdorf, D. J., Solovey, A., Hebbel, R. P. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Origins+of+circulating+endothelial+cells+and+endothelial+outgrowth+from+blood.">Origins of circulating endothelial cells and endothelial outgrowth from blood.</a> J Clin Invest. 105, 71-77 (2000).</li><li>Yoder, M. C., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Redefining+endothelial+progenitor+cells+via+clonal+analysis+and+hematopoietic+stem/progenitor+cell+principals.">Redefining endothelial progenitor cells via clonal analysis and hematopoietic stem/progenitor cell principals.</a> Blood. 109, 1801-1809 (2007).</li><li>Toshner, M., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Transcript+analysis+reveals+a+specific+HOX+signature+associated+with+positional+identity+of+human+endothelial+cells.">Transcript analysis reveals a specific HOX signature associated with positional identity of human endothelial cells.</a> PLOS ONE. 9, e91334 (2014).</li><li>Toshner, M., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Evidence+of+dysfunction+of+endothelial+progenitors+in+pulmonary+arterial+hypertension.">Evidence of dysfunction of endothelial progenitors in pulmonary arterial hypertension.</a> Am J Respir Crit Care Med. 180, 780-787 (2009).</li><li>Wang, J. W., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Analysis+of+the+storage+and+secretion+of+von+Willebrand+factor+in+blood+outgrowth+endothelial+cells+derived+from+patients+with+von+Willebrand+disease.">Analysis of the storage and secretion of von Willebrand factor in blood outgrowth endothelial cells derived from patients with von Willebrand disease.</a> Blood. 121, 2762-2772 (2013).</li><li>O'Neill, C. L., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Therapeutic+revascularisation+of+ischaemic+tissue:+the+opportunities+and+challenges+for+therapy+using+vascular+stem/progenitor+cells.">Therapeutic revascularisation of ischaemic tissue: the opportunities and challenges for therapy using vascular stem/progenitor cells.</a> Stem Cell Res &amp; Ther. 3, 31 (2012).</li><li>Geti, I., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+Practical+and+Efficient+Cellular+Substrate+for+the+Generation+of+Induced+Pluripotent+Stem+Cells+from+Adults:+Blood-Derived+Endothelial+Progenitor+Cells.">A Practical and Efficient Cellular Substrate for the Generation of Induced Pluripotent Stem Cells from Adults: Blood-Derived Endothelial Progenitor Cells.</a> Stem Cells TM. 1, 855-865 (2012).</li><li>Prasain, N., Meador, J. L., Yoder, M. C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Phenotypic+and+functional+characterization+of+endothelial+colony+forming+cells+derived+from+human+umbilical+cord+blood.">Phenotypic and functional characterization of endothelial colony forming cells derived from human umbilical cord blood.</a> Journal of Vis Exp: JoVE. , (2012).</li><li>Martin-Ramirez, J., Hofman, M., van den Biggelaar, M., Hebbel, R. P., Voorberg, J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Establishment+of+outgrowth+endothelial+cells+from+peripheral+blood.">Establishment of outgrowth endothelial cells from peripheral blood.</a> Nat Prot. 7, 1709-1715 (2012).</li><li>Hofmann, N. A., Reinisch, A., Strunk, D. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Isolation+and+large+scale+expansion+of+adult+human+endothelial+colony+forming+progenitor+cells.">Isolation and large scale expansion of adult human endothelial colony forming progenitor cells.</a> Journal of Vis Exp: JoVE. , (2009).</li></ol>

The authors have nothing to disclose.

We present a detailed protocol that allows for the robust and efficient derivation of BOECs from adult peripheral blood mononuclear cells (PBMNCs). Our protocol includes two important refinements that represent advances on previous methods of BOEC isolation.14-16 These include the absence of heparin in the initial PBMNC culture medium and the use of defined, embryonic stem cell-qualified serum. This latter refinement is of particular importance. Embryonic stem cell (ESC)-qualified serum is a more consistent grade of serum and, although it is not known yet what component(s) are enriched in the serum that benefit BOEC isolation, the impact of this defined serum on the efficiency of BOEC generation is clear in our hands. In addition, we have also had success in isolating BOECs using human serum, thereby allowing for the generation of BOECs for clinical translation. In our hands, this refined protocol results in the successful isolation of stable BOEC cultures from greater than 90% of donors, making it one of the most reliable BOEC generation methods reported thus far. Although the use of particular sera is critical to BOEC generation, it also represents a primary limitation of the current protocol. Future improvements to the technique could include the generation of these cells in serum-free, defined culture conditions.
Critical Steps in the protocol include processing blood samples as soon as possible after collection, complete harvesting of the buffy coat cells after density gradient centrifugation and the timely passaging of initial colonies from P0 to P1. This passaging step is critical to establishment of a stable isolation. Like other endothelial cells, BOECs appear to be very sensitive to plating density. If the plating density after passaging is too low, the BOECs will not proliferate. Conversely, if the colonies are allowed to become overconfluent before passaging, the cells will also cease to proliferate and have the tendency to convert into an elongated, mesenchymal cell phenotype. If few colonies appear from days 7 to 14, or if the colonies are small in size, troubleshooting can include increasing cell density by passaging P0 colonies into a T-25 flask instead of a T-75.
Once the technique is mastered, the resultant BOECs can be used in several applications, including in vitro studies of endothelial cell biology, disease modeling and drug screening, as well as in vivo cell transplantation therapies. An important consideration for the development of any cell therapy process is to use cells that are free from pathogenic mutations. We have previously shown that BOECs isolated using our protocol possess genomes that are free from copy number variations and are thus representative of the individual from which they were collected. In addition, we have also demonstrated that the majority of BOEC-derived iPSC lines are free from copy number variations.13 This contrasts with previous reports of copy number variation in fibroblast-derived iPSCs. To date, these cells remain the only iPSCs for which this degree of genomic fidelity has been reported. This feature is important for the field of iPSC biology and the use of iPSCs in disease modeling, drug screening and future cell transplantation therapies.

Until recently, the post-natal generation of new blood vessels was believed to occur exclusively through a process known as angiogenesis, defined as the sprouting of new vessels from the endothelial cells of pre-existing vessels.1 This process contrasts from the vasculogenesis, or the de novo formation of blood vessels from endothelial progenitors, which was thought to occur exclusively during embryogenesis.2 However, more recent studies have identified and isolated circulating endothelial progenitor cells (EPCs) in the peripheral blood of adults. These cells possess the capacity to differentiate into mature endothelial cells in culture and are believed to participate in postnatal vasculogenesis.3,4
Protocols for the isolation and expansion of these EPCs typically involve the culture of peripheral blood mononuclear cells (PBMNCs) in media containing endothelial growth factors, including vascular endothelial growth factor (VEGF) and fibroblast growth factor-2.5-8 EPC cultures produce a variety of dramatically different cell types. Initial cultures (&#60;7 days) are dominated by a monocytic cell type, known in the literature as &#34;early&#34; EPCs. Despite their name, these cells express the monocyte marker CD14, are negative for the progenitor marker CD34 and express only minimal levels of the classical endothelial markers CD31 and VEGF receptor 2 (VEGFR2).5 Continued culture gives rise to a secondary population of cells, known as late outgrowth EPCs or blood outgrowth endothelial cells (BOECs), which appear as discreet colonies of endothelial-like cells. Unlike the monocytic early EPCs, BOECs, which have also been called endothelial colony forming cells (ECFCs), outgrowth endothelial cells or late-outgrowth endothelial cells, exhibit the cobblestone morphology that is typical of endothelial cell monolayers and are highly similar in surface marker5 and gene expression9 to mature endothelial cells.
The generation of endothelial-like cells from peripheral blood offers several advantages, particularly for the study of the endothelial cell dysfunction associated with vascular disorders such as pulmonary arterial hypertension (PAH)10 or von Willebrand disease.11 Prior to the availability of BOECs, endothelial cells could only be derived from explanted organs at time of death or organ transplantation, or isolated from the umbilical vein at birth. This reduced availability represented a serious limitation to understanding the biology of endothelial cells from patients with cardiovascular disorders, as well as the interactions between endothelial cells and either blood cells or mural cells. Furthermore, isolating and culturing a pure population of endothelial cells from these sources is technically challenging and the cells derived by these methods exhibit only a limited proliferative capacity. BOECs therefore offer a valuable surrogate for the isolation and culture of patient-derived primary endothelial cells.
In addition to their in vitro applications, BOECs are also potentially useful in autologous cell transplantation therapies. These applications include both endothelial cell transplantation to promote neovascularization (see 12 and references therein), as well as the generation of induced pluripotent stem cells (iPSCs).13 BOEC-derived iPSCs can be used for disease modeling and offer immense potential as the starting material for autologous cell therapies. BOECs reprogram faster and with a higher efficiency than skin fibroblasts. Furthermore, BOECs also allow for the generation of iPSCs that are free of karyotypic abnormalities, which is an essential feature of any technology that will be suitable for translational applications. The ability to generate iPSCs from a patient blood sample also eliminates the need for a skin biopsy and the generation of skin fibroblasts, thereby facilitating the generation of cells from patients with wound healing disorders, or the very young.
The protocol detailed below, approved by and conducted in accordance with guidelines of the National Research Ethics Service Committee (East of England), provides a simple and reliable method for the generation of BOECs with greater than 90% efficiency from a relatively small volume (60 ml) of peripheral blood. These cells are highly proliferative and can be passaged repeatedly, allowing for the generation of hundreds of millions of cells from a single blood sample.

<table>
	<tbody>
		<tr>
			<td colspan="4">For blood collection</td>
		</tr>
		<tr>
			<td>60 mL syringe with luer-lok tip</td>
			<td>BD</td>
			<td>309653</td>
			<td></td>
		</tr>
		<tr>
			<td>19G Surflo Winged Infusion Set</td>
			<td>Terumo</td>
			<td>SV-19BL</td>
			<td></td>
		</tr>
		<tr>
			<td>50 mL conical centrifuge tube</td>
			<td>StarLab</td>
			<td>E1450</td>
			<td>2 per donor</td>
		</tr>
		<tr>
			<td>Sodium Citrate</td>
			<td>Martindale Pharmaceuticals</td>
			<td>270541</td>
			<td></td>
		</tr>
		<tr>
			<td>Name</td>
			<td>Company</td>
			<td>Catalog Number</td>
			<td>Comments</td>
		</tr>
		<tr>
			<td colspan="4">For buffy coat isolation</td>
		</tr>
		<tr>
			<td>Ficoll-Paque Plus</td>
			<td>GE Healthcare</td>
			<td>17-1440-03</td>
			<td></td>
		</tr>
		<tr>
			<td>Dulbecco&#8217;s PBS (without Ca2+ and Mg2+)</td>
			<td>Sigma-Aldrich</td>
			<td>D8537</td>
			<td></td>
		</tr>
		<tr>
			<td>Sterile wrapped plastic transfer pipettes</td>
			<td>Appleton Woods</td>
			<td>KC231</td>
			<td></td>
		</tr>
		<tr>
			<td>Turk&#8217;s Solution</td>
			<td>Millipore</td>
			<td>1.093E+09</td>
			<td></td>
		</tr>
		<tr>
			<td>Name</td>
			<td>Company</td>
			<td>Catalog Number</td>
			<td>Comments</td>
		</tr>
		<tr>
			<td colspan="4">For cell culture, passaging and freezing cells</td>
		</tr>
		<tr>
			<td>Type 1 Collagen (derived from rat tail)</td>
			<td>BD Biosciences</td>
			<td>35-4236</td>
			<td></td>
		</tr>
		<tr>
			<td>Dulbecco&#8217;s PBS (without Ca2+ and Mg2+)</td>
			<td>Sigma-Aldrich</td>
			<td>D8537</td>
			<td></td>
		</tr>
		<tr>
			<td>0.02M Acetic Acid&#160;</td>
			<td>Sigma-Aldrich</td>
			<td>A6283</td>
			<td>prepared in reagent grade water</td>
		</tr>
		<tr>
			<td>Endothelial Growth Medium-2MV 
			(containing Bullet Kit, but not serum)</td>
			<td>Lonza</td>
			<td>CC-3202</td>
			<td>Note: It is essential that the medium does not contain heparin.&#160;&#160; 
			Do not use EGM-2.</td>
		</tr>
		<tr>
			<td>Fetal Bovine Serum (U.S.), Defined</td>
			<td>Hyclone</td>
			<td>SH30070</td>
			<td></td>
		</tr>
		<tr>
			<td>10x Trypsin EDTA</td>
			<td>Gibco</td>
			<td>T4174</td>
			<td>Dilute to 1x in PBS prior to use</td>
		</tr>
		<tr>
			<td>Heat Inactivated FBS</td>
			<td>Gibco</td>
			<td>10500-064</td>
			<td></td>
		</tr>
		<tr>
			<td>DMEM</td>
			<td>Gibco</td>
			<td>41965-039</td>
			<td></td>
		</tr>
		<tr>
			<td>DMSO</td>
			<td>Sigma-Aldrich</td>
			<td>276855</td>
			<td></td>
		</tr>
		<tr>
			<td>Nalgene Mr. Frosty Freezing Container</td>
			<td>Sigma-Aldrich</td>
			<td>C1562</td>
			<td></td>
		</tr>
		<tr>
			<td>Name</td>
			<td>Company</td>
			<td>Catalog Number</td>
			<td>Comments</td>
		</tr>
		<tr>
			<td colspan="4">For flow cytometric characterization</td>
		</tr>
		<tr>
			<td>FITC-conjugated mouse anti-human CD14</td>
			<td>BD Biosciences</td>
			<td>555397</td>
			<td>Mouse IgG1k, Clone: WM59 
			Dilution: 1:20</td>
		</tr>
		<tr>
			<td>FITC-conjugated mouse anti-human CD31</td>
			<td>BD Biosciences</td>
			<td>555445</td>
			<td>Mouse IgG1k, Clone: WM59 
			Dilution: 1:20</td>
		</tr>
		<tr>
			<td>APC-conjugated mouse anti-human CD34</td>
			<td>BD Biosciences</td>
			<td>555824</td>
			<td>Mouse IgG1k, Clone: 581/CD34 
			Dilution: 1:20</td>
		</tr>
		<tr>
			<td>FITC-conjugated mouse anti-human CD45</td>
			<td>BD Biosciences</td>
			<td>560976</td>
			<td>Mouse IgG1k, Clone: HI30 
			Dilution: 1:20</td>
		</tr>
		<tr>
			<td>&#160;APC-conjugated mouse anti-human VEGFR2</td>
			<td>R&#38;D Systems</td>
			<td>FAB357A</td>
			<td>Mouse IgG1, Clone: 89106 
			Dilution: 1:10</td>
		</tr>
		<tr>
			<td>FITC-conjugated mouse IgG1k isotype control</td>
			<td>BD Biosciences</td>
			<td>555748</td>
			<td>Clone: MOPC-21 
			Dilution: 1:20</td>
		</tr>
		<tr>
			<td>APC-conjugated mouse IgG1k isotype control</td>
			<td>BD Biosciences</td>
			<td>555751</td>
			<td>Clone: MOPC-21 
			Dilution: 1:20</td>
		</tr>
		<tr>
			<td>APC-conjugated mouse IgG1k isotype control</td>
			<td>R&#38;D Systems</td>
			<td>IC002A 
			Dilution: 1:10</td>
			<td>Clone: 11711</td>
		</tr>
		<tr>
			<td>EDTA, 0.5M solution</td>
			<td>Sigma-Aldrich</td>
			<td>E7889</td>
			<td></td>
		</tr>
		<tr>
			<td>Name</td>
			<td>Company</td>
			<td>Catalog Number</td>
			<td>Comments</td>
		</tr>
		<tr>
			<td colspan="4">For immunofluorescent microscopy&#160;</td>
		</tr>
		<tr>
			<td>Corning Costar 24-well tissue culture plate</td>
			<td>Sigma-Aldrich</td>
			<td>CLS3527</td>
			<td></td>
		</tr>
		<tr>
			<td>Paraformaldehyde</td>
			<td>Sigma-Aldrich</td>
			<td>158127</td>
			<td></td>
		</tr>
		<tr>
			<td>BSA</td>
			<td>Sigma-Aldrich</td>
			<td>A7906</td>
			<td></td>
		</tr>
		<tr>
			<td>Polysorbate 20</td>
			<td>Sigma-Aldrich</td>
			<td>P2287</td>
			<td></td>
		</tr>
		<tr>
			<td>Monoclonal mouse anti-human CD34 antibody</td>
			<td>R&#38;D Systems</td>
			<td>MAB72271</td>
			<td>Clone 756510, IgG1, use at 10 &#956;g/ml</td>
		</tr>
		<tr>
			<td>Polyclonal goat anti-human VE-cadherin (CD144)</td>
			<td>R&#38;D Systems</td>
			<td>AF938</td>
			<td>Antigen affinity- purified IgG, use at 1:300</td>
		</tr>
		<tr>
			<td>Monoclonal rabbit anti-human Von Willebrand Factor (vWF)</td>
			<td>Abcam</td>
			<td>ab154193</td>
			<td>Clone EPSISR15, use at 1:250</td>
		</tr>
		<tr>
			<td>Donkey anti-mouse IgG (H+L) secondary antibody, Alexa Fluor 488 conjugate</td>
			<td>Life Technologies</td>
			<td>A-21202</td>
			<td>Polyclonal, 2 mg/ml, use at 1:200</td>
		</tr>
		<tr>
			<td>Donkey anti-goat IgG (H+L) secondary antibody, Alexa Fluor 488 conjugate</td>
			<td>Life Technologies</td>
			<td>A-11055</td>
			<td>Polyclonal, 2 mg/ml, 1:200</td>
		</tr>
		<tr>
			<td>Donkey anti-rabbit IgG (H+L) secondary antibody, Alexa Fluor 568 conjugate</td>
			<td>Life Technologies</td>
			<td>A-10042</td>
			<td>Polyclonal,&#160; 2 mg/ml, 1:200</td>
		</tr>
		<tr>
			<td>DAPI (4&#8242;,6-Diamidino-2-phenylindole dihydrochloride)</td>
			<td>Sigma-Aldrich</td>
			<td>D9542</td>
			<td>use at 1 &#956;g/ml</td>
		</tr>
	</tbody>
</table>

generation and culture of blood outgrowth endothelial cells from human peripheral blood

Historically, the limited availability of primary endothelial cells from patients with vascular disorders has hindered the study of the molecular mechanisms underlying endothelial dysfunction in these individuals. However, the recent identification of blood outgrowth endothelial cells (BOECs), generated from circulating endothelial progenitors in adult peripheral blood, may circumvent this limitation by offering an endothelial-like, primary cell surrogate for patient-derived endothelial cells. Beyond their value to understanding endothelial biology and disease modeling, BOECs have potential uses in endothelial cell transplantation therapies. They are also a suitable cellular substrate for the generation of induced pluripotent stem cells (iPSCs) via nuclear reprogramming, offering a number of advantages over other cell types. We describe a method for the reliable generation, culture and characterization of BOECs from adult peripheral blood for use in these and other applications. This approach (i) allows for the generation of patient-specific endothelial cells from a relatively small volume of adult peripheral blood and (ii) produces cells that are highly similar to primary endothelial cells in morphology, cell signaling and gene expression.

Isolation of buffy coat mononuclear cells from 60 ml of blood typically yields 100-150x106 total white blood cells. When plated into a single T-75 flask, the large number of cells in the unlysed cell suspension makes it difficult to resolve individual adherent cells using brightfield microscopy. Repeated medium changes result in the clearance of non-adherent cells and allow for the visualization of the adherent population of monocytic &#34;early&#34; EPCs. At day 7, the T-75 will contain approximately 7x106 of these elongated adherent cells. From day 7 to 14, colonies of BOECs should appear within the flask (Figure 2A). Colonies first appear as 3 to 5 adjacent cells. Outgrowth colony number can vary from 1 to 10 colonies per 60 ml of blood. Generally, younger donors (i.e., 20-25 years old) tend to produce a greater number of outgrowth colonies, which also appear earlier in culture. BOECs proliferate from this central group of cells to form circular colonies consisting of several hundred cells. Cells within these colonies exhibit a classic endothelial cobblestone morphology.
It is preferable to passage initial colonies when they contain approximately 1000 cells per colony. Outgrowth colonies typically reach this size 7 days after their original appearance in culture. Once the original colonies are passaged into a new T-75 flask, they should proliferate to form a confluent monolayer (3-5x106 cells per flask) within 5 days or less (Figure 2B). In a small percentage of isolations (&#60;10%), outgrowth colonies fail to appear, or do not proliferate sufficiently following this initial passaging step. BOECs that exhibit low proliferation after their first passaging rarely go on to become stable BOEC isolations and often stop proliferating within two to three passages. The monocytic early EPCs contained within the BOEC cultures are non-proliferative and are typically cleared from the cultures within 1-2 passages. Clearance of these early cells is due to cell death, failure of the early cells to re-adhere after passaging and dilution of the non-proliferative early EPCs with repeated passaging.
Passage 1 cells can either be passaged further in culture or frozen down for later use. Once a stable isolation is generated, cells can be passaged at a rate of 1 confluent flask to 3-5 new T-75 flasks up until passage 8 or 9 before becoming quiescent. Again, cell density is critical throughout culture. In our experience, no fewer than 750,000 cells should be plated in a T-75 flask, as lower cell densities can cause growth arrest. Despite the high proliferative potential of BOECs, cells should also not be allowed to become overconfluent (i.e., &#62;5x106 cells per flask) as this can cause conversion of BOECs to a non-proliferative phenotype.
We propose that any cell being labeled as a BOEC should display appropriate cell surface and intracellular staining for endothelial markers. Characterization of BOECs can be achieved by flow cytometry (Figure 3) or fluorescence microscopy (Figure 4), following staining for typical endothelial cell markers. BOECs are positive for the endothelial surface markers CD31 and VEGFR2 and are negative for the monocyte marker CD14 and the pan-leukocyte marker CD45. BOECs also posess Weibel-Palade bodies and thus express Von Willebrand Factor (vWF) as discrete, punctate cytoplasmic staining. Unlike other mature endothelial cell types, such as pulmonary artery or aortic endothelial cells, BOECs also express the progenitor and activation marker CD34 on their surface.
<img alt="Figure 1" src="/files/ftp_upload/53384/53384fig1.jpg" /> 
Figure 1. Schematic diagram of BOEC generation protocol. Peripheral blood mononuclear cells are isolated from venous blood by density gradient centrifugation and cultured on collagen-coated plates in endothelial growth medium containing defined FBS. BOEC colonies appear within 7-14 days of culture. <a href="https://www.jove.com/files/ftp_upload/53384/53384fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" src="/files/ftp_upload/53384/53384fig2.jpg" /> 
Figure 2. Brightfield images of representative BOEC cultures. (A) Outgrowth colonies appear in cultures between days 7 and 14. Colonies present as collections of endothelial-like cells, which are arranged in a cobblestone monolayer and proliferate radially out from a central point. Surrounding the outgrowth colonies are the adherent monocytic cells that make up the vast majority of cells in early cultures. These cells, previously described as &#34;early&#34; endothelial progenitor cells, have a spindle-like morphology and express the monocytic marker CD14. (B) Following passaging, the highly proliferative BOECs take over cultures, as the non-proliferative monocytic cells either die off or fail to re-attach after passaging. Scale bar 250&#956;m. <a href="https://www.jove.com/files/ftp_upload/53384/53384fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" src="/files/ftp_upload/53384/53384fig3.jpg" /> 
Figure 3. Characterization of BOECs by flow cytometry. BOECs were trypsinized and stained with fluorescently-conjugated isotype control antibodies (grey filled peak) or antibodies directed against specific surface markers (red line). Surface markers for cytometric characterization include the hematopoietic markers CD45 and CD14, the endothelial markers CD31 and VEGFR2 and the progentior and endothelial activation marker CD34. <a href="https://www.jove.com/files/ftp_upload/53384/53384fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" src="/files/ftp_upload/53384/53384fig4.jpg" /> 
Figure 4. Immunofluorescent staining of BOECs for endothelial cell markers. Representative immunofluorescence images of BOECs immunostained with antibodies directed against endothelial cell surface marker CD144 (VE-cadherin, top right panel) and the blood glycoprotein von Willebrand Factor (vWF, bottom right panel). Corresponding panels showing nuclear DAPI staining are shown to the left. Scale bar 50&#956;m. for CD144. <a href="https://www.jove.com/files/ftp_upload/53384/53384fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about Generation and Culture of Blood Outgrowth Endothelial Cells from Human Peripheral Blood at JoVE.com

Generation and Culture of Blood Outgrowth Endothelial Cells from Human Peripheral Blood

This protocol allows for the reliable generation and characterization of blood outgrowth endothelial cells (BOECs) from a small volume of adult peripheral blood. BOECs can be used as a surrogate for endothelial cells from patients with vascular disorders and as a substrate for the generation of induced pluripotent stem cells.

Historically, the limited availability of primary endothelial cells from patients with vascular disorders has hindered the study of the molecular ...

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18.9K Views.  University of Cambridge. This protocol allows for the reliable generation and characterization of blood outgrowth endothelial cells (BOECs) from a small volume of adult peripheral blood. BOECs can be used as a surrogate for endothelial cells from patients with vascular disorders and as a substrate for the generation of induced pluripotent stem cells.

Video: Generation and Culture of Blood Outgrowth Endothelial Cells from Human Peripheral Blood

Enrichment of NK Cells from Human Blood with the RosetteSep Kit from StemCell Technologies

Natural killer (NK) cells are large granular cytotoxic lymphocytes that belong to the innate immune system and play major roles in fighting against cancer and infections, but are also implicated in the early stages of pregnancy and transplant rejection. These cells are present in peripheral blood, from which they can be isolated. Cells can be isolated using either positive or negative selection. For positive selection we use antibodies directed to a surface marker present only on the cells of interest whereas for negative selection we use cocktails of antibodies targeted to surface markers present on all cells but the cells of interest. This latter technique presents the advantage of leaving the cells of interest free of antibodies, thereby reducing the risk of unwanted cell activation or differenciation. In this video-protocol we demonstrate how to separate NK cells from human blood by negative selection, using the RosetteSep kit from StemCell technologies. The procedure involves obtaining human peripheral blood (under an institutional review board-approved protocol to protect the human subjects) and mixing it with a cocktail of antibodies that will bind to markers absent on NK cells, but present on all other mononuclear cells present in peripheral blood (e.g., T lymphocytes, monocytes...). The antibodies present in the cocktail are conjugated to antibodies directed to glycophorin A on erythrocytes. All unwanted cells and red blood cells will therefore be trapped in complexes. The mix of blood and antibody cocktail is then diluted, overlayed on a Histopaque gradient, and centrifuged. NK cells (&gt;80% pure) can be collected at the interface between the Histopaque and the diluted plasma. Similar cocktails are available for enrichment of other cell populations, such as human T lymphocytes.

Natural killer cells are a small population of lymphocytes. Here we show how to isolate these cells from human blood by negative selection, using a kit from StemCell Technologies. The cells obtained are viable and untouched by antibodies, and therefore ready to be used for a number of procedures.

Natural killer (NK) cells are large granular cytotoxic lymphocytes that belong to the innate immune system and play major roles in fighting against cancer ...

Isolation and Culture of Pulmonary Endothelial Cells from Neonatal Mice

Endothelial cells provide a useful research model in many areas of vascular biology. Since its first isolation 1, human umbilical vein endothelial cells (HUVECs) have shown to be convenient, easy to obtain and culture, and thus are the most widely studied endothelial cells. However, for research focused on processes like angiogenesis, permeability or many others, microvascular endothelial cells (ECs) are a much more physiologically relevant model to study 2. Furthermore, ECs isolated from knockout mice provide a useful tool for analysis of protein function ex vivo. Several approaches to isolate and culture microvascular ECs of different origin have been reported to date 3-7, but consistent isolation and culture of pure ECs is still a major technical problem in many laboratories. Here, we provide a step-by-step protocol on a reliable and relatively simple method of isolating and culturing mouse lung endothelial cells (MLECs). In this approach, lung tissue obtained from 6- to 8-day old pups is first cut into pieces, digested with collagenase/dispase (C/D) solution and dispersed mechanically into single-cell suspension. MLECS are purified from cell suspension using positive selection with anti-PECAM-1 antibody conjugated to Dynabeads using a Magnetic Particle Concentrator (MPC). Such purified cells are cultured on gelatin-coated tissue culture (TC) dishes until they become confluent. At that point, cells are further purified using Dynabeads coupled to anti-ICAM-2 antibody. MLECs obtained with this protocol exhibit a cobblestone phenotype, as visualized by phase-contrast light microscopy, and their endothelial phenotype has been confirmed using FACS analysis with anti-VE-cadherin 8 and anti-VEGFR2 9 antibodies and immunofluorescent staining of VE-cadherin. In our hands, this two-step isolation procedure consistently and reliably yields a pure population of MLECs, which can be further cultured. This method will enable researchers to take advantage of the growing number of knockout and transgenic mice to directly correlate in vivo studies with results of in vitro experiments performed on isolated MLECs and thus help to reveal molecular mechanisms of vascular phenotypes observed in vivo.

Here, we describe a protocol for isolation and culture of murine pulmonary endothelial cells. This method comprises mechanic and enzymatic lung tissue dissociation as well as a 2-step purification process using anti-PECAM-1 and anti-ICAM-2 antibodies conjugated to magnetic beads, which produces a pure endothelial cell population of mostly microvascular origin.

Endothelial cells provide a useful research model in many areas of vascular biology. Since its first isolation 1, human umbilical vein endothelial cells ...

Phenotypic and Functional Characterization of Endothelial Colony Forming Cells Derived from Human Umbilical Cord Blood

Longstanding views of new blood vessel formation via angiogenesis, vasculogenesis, and arteriogenesis have been recently reviewed1. The presence of circulating endothelial progenitor cells (EPCs) were first identified in adult human peripheral blood by Asahara et al. in 1997 2 bringing an infusion of new hypotheses and strategies for vascular regeneration and repair. EPCs are rare but normal components of circulating blood that home to sites of blood vessel formation or vascular remodeling, and facilitate either postnatal vasculogenesis, angiogenesis, or arteriogenesis largely via paracrine stimulation of existing vessel wall derived cells3. No specific marker to identify an EPC has been identified, and at present the state of the field is to understand that numerous cell types including proangiogenic hematopoietic stem and progenitor cells, circulating angiogenic cells, Tie2+ monocytes, myeloid progenitor cells, tumor associated macrophages, and M2 activated macrophages participate in stimulating the angiogenic process in a variety of preclinical animal model systems and in human subjects in numerous disease states4, 5. Endothelial colony forming cells (ECFCs) are rare circulating viable endothelial cells characterized by robust clonal proliferative potential, secondary and tertiary colony forming ability upon replating, and ability to form intrinsic in vivo vessels upon transplantation into immunodeficient mice6-8. While ECFCs have been successfully isolated from the peripheral blood of healthy adult subjects, umbilical cord blood (CB) of healthy newborn infants, and vessel wall of numerous human arterial and venous vessels 6-9, CB possesses the highest frequency of ECFCs7 that display the most robust clonal proliferative potential and form durable and functional blood vessels in vivo8, 10-13. While the derivation of ECFC from adult peripheral blood has been presented14, 15, here we describe the methodologies for the derivation, cloning, expansion, and in vitro as well as in vivo characterization of ECFCs from the human umbilical CB.

Endothelial colony forming cells (ECFCs) are circulating endothelial cells with robust clonal proliferative potential that display intrinsic in vivo vessel forming ability. Phenotypic and functional characterization of outgrowth endothelial cells derived from CB are important to identify and isolate bona fide ECFCs for potential clinical application in repairing damaged tissues.

Longstanding views of new blood vessel formation via angiogenesis, vasculogenesis, and arteriogenesis have been recently reviewed1. The presence of ...

Generation of Human Induced Pluripotent Stem Cells from Peripheral Blood Using the STEMCCA Lentiviral Vector

Through the ectopic expression of four transcription factors, Oct4, Klf4, Sox2 and cMyc, human somatic cells can be converted to a pluripotent state, generating so-called induced pluripotent stem cells (iPSCs)1-4. Patient-specific iPSCs lack the ethical concerns that surround embryonic stem cells (ESCs) and would bypass possible immune rejection. Thus, iPSCs have attracted considerable attention for disease modeling studies, the screening of pharmacological compounds, and regenerative therapies5.
We have shown the generation of transgene-free human iPSCs from patients with different lung diseases using a single excisable polycistronic lentiviral Stem Cell Cassette (STEMCCA) encoding the Yamanaka factors6. These iPSC lines were generated from skin fibroblasts, the most common cell type used for reprogramming. Normally, obtaining fibroblasts requires a skin punch biopsy followed by expansion of the cells in culture for a few passages. Importantly, a number of groups have reported the reprogramming of human peripheral blood cells into iPSCs7-9. In one study, a Tet inducible version of the STEMCCA vector was employed9, which required the blood cells to be simultaneously infected with a constitutively active lentivirus encoding the reverse tetracycline transactivator. In contrast to fibroblasts, peripheral blood cells can be collected via minimally invasive procedures, greatly reducing the discomfort and distress of the patient. A simple and effective protocol for reprogramming blood cells using a constitutive single excisable vector may accelerate the application of iPSC technology by making it accessible to a broader research community. Furthermore, reprogramming of peripheral blood cells allows for the generation of iPSCs from individuals in which skin biopsies should be avoided (i.e. aberrant scarring) or due to pre-existing disease conditions preventing access to punch biopsies.
Here we demonstrate a protocol for the generation of human iPSCs from peripheral blood mononuclear cells (PBMCs) using a single floxed-excisable lentiviral vector constitutively expressing the 4 factors. Freshly collected or thawed PBMCs are expanded for 9 days as described10,11 in medium containing ascorbic acid, SCF, IGF-1, IL-3 and EPO before being transduced with the STEMCCA lentivirus. Cells are then plated onto MEFs and ESC-like colonies can be visualized two weeks after infection. Finally, selected clones are expanded and tested for the expression of the pluripotency markers SSEA-4, Tra-1-60 and Tra-1-81. This protocol is simple, robust and highly consistent, providing a reliable methodology for the generation of human iPSCs from readily accessible 4 ml of blood.

Here we show a simple and effective protocol for the generation of human iPSCs from 3-4 ml of peripheral blood using a single lentiviral reprogramming vector. Reprogramming of readily available blood cells promises to accelerate the utilization of iPSC technology by making it accessible to a broader research community.

Through the ectopic expression of four transcription factors, Oct4, Klf4, Sox2 and cMyc, human somatic cells can be converted to a pluripotent state, ...

Purification and microRNA Profiling of Exosomes Derived from Blood and Culture Media

Stable miRNAs are present in all body fluids and some circulating miRNAs are protected from degradation by sequestration in small vesicles called exosomes. Exosomes can fuse with the plasma membrane resulting in the transfer of RNA and proteins to the target cell. Their biological functions include immune response, antigen presentation, and intracellular communication. Delivery of miRNAs that can regulate gene expression in the recipient cells via blood has opened novel avenues for target intervention. In addition to offering a strategy for delivery of drugs or RNA therapeutic agents, exosomal contents can serve as biomarkers that can aid in diagnosis, determining treatment options and prognosis.	Here we will describe the procedure for quantitatively analyzing miRNAs and messenger RNAs (mRNA) from exosomes secreted in blood and cell culture media. Purified exosomes will be characterized using western blot analysis for exosomal markers and PCR for mRNAs of interest. Transmission electron microscopy (TEM) and immunogold labeling will be used to validate exosomal morphology and integrity. Total RNA will be purified from these exosomes to ensure that we can study both mRNA and miRNA from the same sample. After validating RNA integrity by Bioanalyzer, we will perform a medium throughput quantitative real time PCR (qPCR) to identify the exosomal miRNA using Taqman Low Density Array (TLDA) cards and gene expression studies for transcripts of interest.	
 These protocols can be used to quantify changes in exosomal miRNAs in patients, rodent models and cell culture media before and after pharmacological intervention. Exosomal contents vary due to the source of origin and the physiological conditions of cells that secrete exosomes. These variations can provide insight on how cells and systems cope with stress or physiological perturbations. Our representative data show variations in miRNAs present in exosomes purified from mouse blood, human blood and human cell culture media.	
 Here we will describe the procedure for quantitatively analyzing miRNAs and messenger RNAs (mRNA) from exosomes secreted in blood and cell culture media. Purified exosomes will be characterized using western blot analysis for exosomal markers and PCR for mRNAs of interest. Transmission electron microscopy (TEM) and immunogold labeling will be used to validate exosomal morphology and integrity. Total RNA will be purified from these exosomes to ensure that we can study both mRNA and miRNA from the same sample. After validating RNA integrity by Bioanalyzer, we will perform a medium throughput quantitative real time PCR (qPCR) to identify the exosomal miRNA using Taqman Low Density Array (TLDA) cards and gene expression studies for transcripts of interest.
 These protocols can be used to quantify changes in exosomal miRNAs in patients, rodent models and cell culture media before and after pharmacological intervention. Exosomal contents vary due to the source of origin and the physiological conditions of cells that secrete exosomes. These variations can provide insight on how cells and systems cope with stress or physiological perturbations. Our representative data show variations in miRNAs present in exosomes purified from mouse blood, human blood and human cell culture media

The presence of stable microRNAs (miRNAs) in exosomes has generated immense interest as a novel mode of intercellular communication, for their potential utility as biomarkers and as a route for therapeutic intervention. Here we demonstrate exosome purification from blood and culture media followed by quantitative PCR to identify miRNAs being transported.

Stable miRNAs are present in all body fluids and some circulating miRNAs  are protected from degradation by sequestration in small vesicles called  ...

Efficient iPS Cell Generation from Blood Using Episomes and HDAC Inhibitors

This manuscript illustrates a protocol for efficiently creating integration-free human induced pluripotent stem cells (iPSCs) from peripheral blood using episomal plasmids and histone deacetylase (HDAC) inhibitors. The advantages of this approach include: (1) the use of a minimal amount of peripheral blood as a source material; (2) nonintegrating reprogramming vectors; (3) a cost effective method for generating vector free iPSCs; (4) a single transfection; and (5) the use of small molecules to facilitate epigenetic reprogramming. Briefly, peripheral blood mononuclear cells (PBMCs) are isolated from routine phlebotomy samples and then cultured in defined growth factors to yield a highly proliferative erythrocyte progenitor cell population that is remarkably amenable to reprogramming. Nonintegrating, nontransmissible episomal plasmids expressing OCT4, SOX2, KLF4, MYCL, LIN28A, and a p53 short hairpin (sh)RNA are introduced into the derived erythroblasts via a single nucleofection. Cotransfection of an episome that expresses enhanced green fluorescent protein (eGFP) allows for easy identification of transfected cells. A separate replication-deficient plasmid expressing Epstein-Barr nuclear antigen 1 (EBNA1) is also added to the reaction mixture for increased expression of episomal proteins. Transfected cells are then plated onto a layer of irradiated mouse embryonic fibroblasts (iMEFs) for continued reprogramming. As soon as iPSC-like colonies appear at about twelve days after nucleofection, HDAC inhibitors are added to the medium to facilitate epigenetic remodeling. We have found that the inclusion of HDAC inhibitors routinely increases the generation of fully reprogrammed iPSC colonies by 2 fold. Once iPSC colonies exhibit typical human embryonic stem cell (hESC) morphology, they are gently transferred to individual iMEF-coated tissue culture plates for continued growth and expansion.

Here we describe a protocol for generating human induced pluripotent stem cells from peripheral blood using an episome based reprogramming strategy and histone deacetylase inhibitors.

This manuscript illustrates a protocol for efficiently creating integration-free human induced pluripotent stem cells (iPSCs) from peripheral blood using ...

Two-photon Imaging of Intracellular Ca2+ Handling and Nitric Oxide Production in Endothelial and Smooth Muscle Cells of an Isolated Rat Aorta

Calcium is a very important regulator of many physiological processes in vascular tissues. Most endothelial and smooth muscle functions highly depend on changes in intracellular calcium ([Ca2+]i) and nitric oxide (NO). In order to understand how [Ca2+]i, NO and downstream molecules are handled by a blood vessel in response to vasoconstrictors and vasodilators, we developed a novel technique that applies calcium-labeling (or NO-labeling) dyes with two photon microscopy to measure calcium handling (or NO production) in isolated blood vessels. Described here is a detailed step-by-step procedure that demonstrates how to isolate an aorta from a rat, label calcium or NO within the endothelial or smooth muscle cells, and image calcium transients (or NO production) using a two photon microscope following physiological or pharmacological stimuli. The benefits of using the method are multi-fold: 1) it is possible to simultaneously measure calcium transients in both endothelial cells and smooth muscle cells in response to different stimuli; 2) it allows one to image endothelial cells and smooth muscle cells in their native setting; 3) this method is very sensitive to intracellular calcium or NO changes and generates high resolution images for precise measurements; and 4) described approach can be applied to the measurement of other molecules, such as reactive oxygen species. In summary, application of two photon laser emission microscopy to monitor calcium transients and NO production in the endothelial and smooth muscle cells of an isolated blood vessel has provided high quality quantitative data and promoted our understanding of the mechanisms regulating vascular function.

Two-photon Imaging of Intracellular Ca2+ Handling and Nitric Oxide Production in Endothelial and Smooth Muscle Cells of an Isolated Rat Aorta

Vascular cell functiondepends on activity of intracellular messengers. Described here is an ex vivo two photon imaging method that allows the measurement of intracellular calcium and nitric oxide levels in response to physiological and pharmacological stimuli in individual endothelial and smooth muscle cells of an isolated aorta.

Calcium is a very important regulator of many physiological processes in vascular tissues. Most endothelial and smooth muscle functions highly depend on ...

Immunofluorescence Analysis of Endogenous and Exogenous Centromere-kinetochore Proteins

"Centromeres" and "kinetochores" refer to the site where chromosomes associate with the spindle during cell division. Direct visualization of centromere-kinetochore proteins during the cell cycle remains a fundamental tool in investigating the mechanism(s) of these proteins. Advanced imaging methods in fluorescence microscopy provide remarkable resolution of centromere-kinetochore components and allow direct observation of specific molecular components of the centromeres and kinetochores. In addition, methods of indirect immunofluorescent (IIF) staining using specific antibodies are crucial to these observations. However, despite numerous reports about IIF protocols, few discussed in detail problems of specific centromere-kinetochore proteins.1-4 Here we report optimized protocols to stain endogenous centromere-kinetochore proteins in human cells by using paraformaldehyde fixation and IIF staining. Furthermore, we report protocols to detect Flag-tagged exogenous CENP-A proteins in human cells subjected to acetone or methanol fixation. These methods are useful in detecting and quantifying endogenous centromere-kinetochore proteins and Flag-tagged CENP-A proteins, including those in human cells.

Here we report protocols to detect endogenous and exogenous centromere-kinetochore proteins in human cells and quantify these protein levels at centromeres-kinetochores by indirect immunofluorescent staining through the use of fixation (paraformaldehyde, acetone, or methanol fixation).

"Centromeres" and "kinetochores" refer to the site where chromosomes associate with the spindle during cell division. Direct visualization of ...

Isolation and Characterization of Microvesicles from Peripheral Blood

The release of extracellular vesicles (EVs) including small endosomal-derived exosomes (Exos, diameter &#60; 100 nm) and large plasma membrane-derived microvesicles (MVs, diameter &#62; 100 nm) is a fundamental cellular process that occurs in all living cells. These vesicles transport proteins, lipids and nucleic acids specific for their cell of origin and in vitro studies have highlighted their importance as mediators of intercellular communication. EVs have been successfully isolated from various body fluids and especially EVs in blood have been identified as promising biomarkers for cancer or infectious diseases. In order to allow the study of MV subpopulations in blood, we present a protocol for the standardized isolation and characterization of MVs from peripheral blood samples. MVs are pelleted from EDTA-anticoagulated plasma samples by differential centrifugation and typically possess a diameter of 100 - 600 nm. Due to their larger size, they can easily be studied by flow cytometry, a technique that is routinely used in clinical diagnostics and available in most laboratories. Several examples for quality control assays of the isolated MVs will be given and markers that can be used for the discrimination of different MV subpopulations in blood will be presented.

Extracellular vesicles present in blood have been suggested as novel biomarkers for various diseases. Here, we present a protocol for the isolation of large plasma membrane-derived microvesicles from peripheral blood samples and their subsequent analysis by conventional flow cytometry and Western Blotting.

The release of extracellular vesicles (EVs) including small endosomal-derived exosomes (Exos, diameter &#60; 100 nm) and large plasma membrane-derived ...

A Uniform Shear Assay for Human Platelet and Cell Surface Receptors via Cone-plate Viscometry

Many biological cells/tissues sense the mechanical properties of their local environments via mechanoreceptors, proteins that can respond to forces like pressure or mechanical perturbations. Mechanoreceptors detect their stimuli and transmit signals via a great diversity of mechanisms. Some of the most common roles for mechanoreceptors are in neuronal responses, like touch and pain, or hair cells which function in balance and hearing. Mechanosensation is also important for cell types which are regularly exposed to shear stress such as endothelial cells, which line blood vessels, or blood cells which experience shear in normal circulation. Viscometers are devices that detect the viscosity of fluids. Rotational viscometers may also be used to apply a known shear force to fluids. The ability of these instruments to introduce uniform shear to fluids has been exploited to study many biological fluids including blood and plasma. Viscometry may also be used to apply shear to the cells in a solution, and to test the effects of shear on specific ligand-receptor pairs. Here, we utilize cone-plate viscometry to test the effects of endogenous levels of shear stress on platelets treated with antibodies against the platelet mechanosensory receptor complex GPIb-IX.

We describe an in-solution method to apply uniform shear to platelet surface receptors using cone-plate viscometry. This method may also be used more broadly to apply shear to other cell types and cell-fragments and need not target a specific ligand-receptor pair.

Many biological cells/tissues sense the mechanical properties of their local environments via mechanoreceptors, proteins that can respond to forces like ...