We thank Miltenyi Biotec, Germany for providing reagents and CliniMACS Prodigy equipment for evaluation studies. We thank George T. McNamara (Pediatric department, MD Anderson Cancer Center) for proof reading the manuscript. Grant support: Cancer Center Core Grant (CA16672); RO1 (CA124782, CA120956, CA141303; CA141303); R33 (CA116127); P01 (CA148600); Burroughs Wellcome Fund; Cancer Prevention and Research Institute of Texas; CLL Global Research Foundation; Estate of Noelan L. Bibler; Gillson Longenbaugh Foundation; Harry T. Mangurian, Jr., Fund for Leukemia Immunotherapy; Institute of Personalized Cancer Therapy; Leukemia and Lymphoma Society; Lymphoma Research Foundation; MDACC&#8217;s Sister Institution Network Fund; Miller Foundation; Mr. Herb Simons; Mr. and Mrs. Joe H. Scales; Mr. Thomas Scott; National Foundation for Cancer Research; Pediatric Cancer Research Foundation; William Lawrence and Blanche Hughes Children's Foundation.

1. Preparation of Materials under Sterile Conditions (See Materials and Equipment Table)
<ol>
	<li>Prepare 3 L of PBS/EDTA buffer supplemented with human serum albumin (HSA) to a final concentration of 0.5% (w/v).</li>
	<li>Prepare 1 L bag of clinical grade 0.9 % sodium chloride (NaCl) solution and 2 L of GMP grade cell culture medium.</li>
	<li>Prepare 60 nmol of CMV-specific peptide antigen cocktail by reconstituting one vial of CMV pp65 with 8 ml of sterile water.</li>
	<li>Transfer CMV pp65 peptide cocktail into a 50 ml volume freezing bag using a Luer/Spike interconnector and clamp with locking forceps to avoid subsequent distribution of cocktail into the tubing set. Open cell enrichment tubing set (TS 500) under sterile conditions.</li>
	<li>Using sterile tubing welder, connect peptide cocktail freezing bag into tube connection for valve 2 of tubing set TS 500. Do not open the peptide cocktail bag clamp at this time.</li>
	<li>Remove 1 x 109 TNC from starting cellular product and suspend in PBS/EDTA buffer containing 2.5% HSA to a total volume of 50 ml. Inject the cellular product into a 150 ml transfer bag.</li>
</ol>
2. Preparation and Use of Automated Cell Enrichment System (See Materials and Equipment Table)
<ol>
	<li>Switch on the cell enrichment system (Figure 1B) and select the program &#8220; CCS_IFN-&#947; Enrichment&#8221;. Observe a user interface showing screens with instructions and pictures guiding the operator through the procedure.</li>
	<li>Enter the parameter &#8220;Operator&#8221; and &#8220;Tubing Set P/N No&#8221;. Next, install the Tubing Set 500 to automated cell enrichment device as per instructions displayed on the interactive monitor screen.</li>
	<li>Follow the step by step instructions displayed on the screen to connect the medium and buffers to the device. Record catalogue number and lot number of the reagents before connecting to the instrument.</li>
	<li>After the final check of the tubing set, open the clamp of the peptide cocktail bag. Open the medium bag and initiate automatic priming of the tubing set.</li>
	<li>After the priming step is completed, supplement HSA (2.5%) into NaCl buffer in the reservoir bag (200 ml) with the help of the sterile tubing welder. Transfer the starting cellular product into the &#8220;Application bag&#8221; using the sterile tubing welder.</li>
	<li>Connect CCS (IFN&#947;) reagents into respective tubing via adapters. Enter preferred time to collect a fraction of cellular material before enrichment process. Review and verify the accuracy of all data/parameters entered. Start the process.</li>
	<li>Before the start of automated cell enrichment process, remove the Quality Control Bag (QCB, original fraction (ori) contains approximately 1.3 ml out of 100 ml chamber content diluted with PBS/EDTA buffer). Seal the QCB, weigh, and store at 4 &#176;C.</li>
	<li>Start the enrichment process. At the end of the process, target cells will be eluted with an approximate volume of elution buffer from the reservoir bag.</li>
	<li>Seal the Non Target Cell Bag (NTCB, negative fraction = neg) and Target Cell Bag (TCB, positive fraction = pos) and weigh each bag. The weights will be used later for calculation of the cell numbers.</li>
	<li>Immediately after the enrichment procedure collect two aliquots per fraction for flow cytometry analysis, and store the rest of the samples at 4 &#176;C. Use one sample aliquot for cell count determination and the other sample aliquot for the enrichment performance analysis (Table 1).</li>
	<li>Remove the tubing set from the cell enrichment instrument. Transfer the log file to a USB drive for future use. 
	NOTE:&#160; All reagents should be prepared under sterile conditions. The use of a Biosafety type II hood is highly recommended. Use steady-state apheresis cellular product (non-mobilized) isolated from a healthy CMV-seropositive donor to enrich CMV antigen specific T cells. Only FDA licensed HSA should be used. The buffer for cell preparation should be kept at&#160; +19 &#176;C to +25 &#176;C as lower or higher ambient temperatures will result in reduced purity and a reduced yield of the target cells.</li>
</ol>
3. Cell Count Determination
<ol>
	<li>Take the aliquots of QCB , NTCB and TCB for cell counts as shown in Table 1. Add CD45-VoBlue to each aliquot (titer 1:11) and incubate in the dark for 10 min at 4 &#176;C.</li>
	<li>Add 1.5 ml freshly prepared red blood cell lysis solution (1x) to the original fraction and negative fraction, 450 &#181;l freshly prepared red blood cell lysis solution to the positive fraction, and incubate all fractions for 15 min at RT.</li>
	<li>Just prior to analysis, add propidium iodide to a final concentration of 1 &#181;g/ml (1:100 dilution of 100 &#181;g/ml). Use automatic cell counter to determine cell count and viability. Use cell counter device recommended software for flow cytometry analysis. Determine the absolute counts of leukocytes for original, negative and positive fractions. 
	&#160;NOTE: The cell count of viable leukocytes per ml of the samples taken for cell count analysis is determined using the cell analyzer recommended software.</li>
	<li>Set the region as shown in Figure 2 (region 5, viable leukocytes). Use the following gating strategy to determine cell count. A viable leukocyte in original fraction is shown in Figure 2.</li>
	<li>The indicated regions (Figure 2, 1-6) are hierarchically as follows: 
	1: Time gate &#8594; 2: Single cells &#8594; 3: CD45+ cells &#8594; 4: Leukocytes (debris excluded) &#8594; 5: Viable leukocytes&#160;&#8594; 6: Viable lymphocytes</li>
	<li>Repeat the same steps to determine cell counts for negative and positive fractions. Calculate the cell count of the whole fraction by considering the diluent factor of the sample and total volume of the fraction (Table 2).</li>
</ol>
4. Examination of the Separation Performance
<ol>
	<li>Wash the aliquots of QCB, NTCB and TCB fraction cells with pre-chilled PBS/EDTA buffer/0.5% AB serum. Centrifuge the cells at 300 x g for 5 min at 4 &#176;C and aspirate the supernatant.</li>
	<li>Resuspend cells in 100 &#181;l antibody-fluorochrome staining mixture containing: CD3-FITC, CD4-APC, CD8-APC-Vio770, CD14-PerCP, CD20-PerCP, CD45-VioBlue and anti-IFN&#947;-PE (titer 1:11) and incubate in the dark for 10 min at 4 &#176;C.</li>
	<li>Add 1 ml freshly prepared red blood cell lysis solution (1x) and incubate for 15 min at RT. Centrifuge at 300 x g for 5 min at 4 &#176;C and aspirate the supernatant. Resuspend the cells in an adequate volume of PBS/EDTA Buffer/ 0.5% AB Serum.</li>
	<li>Add propidium iodide to a final concentration of 1 &#181;g/ml just prior to analysis (1:100 dilution of 100 &#181;g/ml). Perform flow cytometry analysis to evaluate the purity of the sample.</li>
	<li>Use the following gating strategy to calculate the CD3+ T cells in viable leukocyte Gating strategy for determining the CD3+ T cells is shown in positive fraction after CCS enrichment process. The indicated regions (Figure 3A and 3B, 1-6) are hierarchically linked as follows: 
	1: Time gate &#8594; 2: Single cells &#8594; 3: CD45+ cells &#8594; 4: Cells (debris excluded) &#8594; 5: Viable leukocytes &#8594; 6: Viable CD3+ cells population</li>
	<li>Determine the frequencies of CD4+, CD8+, CD4+ IFN-&#947;+ and CD8+ IFN-&#947;+ T cells after CCS enrichment process (Table 2).</li>
	<li>Use the gating strategy to determine the frequencies of CD4+, CD8+, CD4+ IFN-&#947;+ and CD8+ IFN-&#947;+ T cells shown below for an original and enriched (captured) positive fraction after CCS process. The indicated regions are hierarchically linked and named as follows: 
	1: Time gate &#8594; 2: Single cells&#160;&#8594; 3: CD45+ cells&#160;&#8594; 4: Cells (debris excluded) &#8594; 5: Viable Leukocytes &#8594; 6: Viable CD3+ cells &#8594; 7: CD4+ cells &#8594; 7a: CD4+ IFN-&#947;+ cells (box) &#8594; 8: CD8+ cells &#8594; 8a: CD8+ IFN-&#947;+ cells (box) &#160;</li>
</ol>
NOTE: The first 6 indicated regions of the hierarchy links are the same as Figure 3, (1-6) and last 2 regions are shown in Figure 4 (6-8a).

<ol>
	<li>Syed, B. A., Evans, J. B. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=From+the+Analyst's+Couch+Stem+Cell+Therapy+Market.">From the Analyst's Couch Stem Cell Therapy Market.</a> Nat Rev Drug Discov. 12 (3), 185-186 (2013).</li><li>Maus, M. V., 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=Adoptive+Immunotherapy+for+Cancer+or+Viruses.">Adoptive Immunotherapy for Cancer or Viruses.</a> Annu Rev Immunol. 32, 189-225 (2014).</li><li>Kumaresan, P. R., 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=Bioengineering+T+cells+to+target+carbohydrate+to+treat+opportunistic+fungal+infection.">Bioengineering T cells to target carbohydrate to treat opportunistic fungal infection.</a> Proc Natl Acad Sci U S A. 111 (29), 10660-10665 (2014).</li><li>Singh, H., 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=Redirecting+specificity+of+T-cell+populations+for+CD19+using+the+Sleeping+Beauty+system.">Redirecting specificity of T-cell populations for CD19 using the Sleeping Beauty system.</a> Cancer Res. 68 (8), 2961-2971 (2008).</li><li>Kumaresan, P. 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Rise of Cell-Based Immunotherapy : Personalized Medicine Takes Next Step Forward.</a> Genetic Engineering &amp; Biotechnology News. 33 (5), 12-13 (2013).</li><li>Apel, 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=Integrated+Clinical+Scale+Manufacturing+System+for+Cellular+Products+Derived+by+Magnetic+Cell+Separation,+Centrifugation+and+Cell+Culture.">Integrated Clinical Scale Manufacturing System for Cellular Products Derived by Magnetic Cell Separation, Centrifugation and Cell Culture.</a> Chem-Ing-Tech. 85 (1-2), 103-110 (2013).</li><li>Brestrich, G., 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=Adoptive+T-Cell+Therapy+of+a+Lung+Transplanted+Patient+with+Severe+CMV+Disease+and+Resistance+to+Antiviral+Therapy.">Adoptive T-Cell Therapy of a Lung Transplanted Patient with Severe CMV Disease and Resistance to Antiviral Therapy.</a> Am J Transplant. 9 (7), 1679-1684 (2009).</li><li>Feuchtinger, 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=Clinical+grade+generation+of+hexon-specific+T+cells+for+adoptive+T-cell+transfer+as+a+treatment+of+adenovirus+infection+after+allogeneic+stem+cell+transplantation.">Clinical grade generation of hexon-specific T cells for adoptive T-cell transfer as a treatment of adenovirus infection after allogeneic stem cell transplantation.</a> J Immunother. 31 (2), 199-206 (2008).</li><li>Peggs, K. 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M., Remberger, M., Alvin, O., Karlsson, H., Ringden, O. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Increased+Costs+after+Allogeneic+Haematopoietic+Sct+Are+Associated+with+Major+Complications+and+Re-Transplantation.">Increased Costs after Allogeneic Haematopoietic Sct Are Associated with Major Complications and Re-Transplantation.</a> Biol Blood Marrow Transplant. 18 (2), S339-S339 (2012).</li><li>Leen, A. 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=Multicenter+study+of+banked+third-party+virus-specific+T+cells+to+treat+severe+viral+infections+after+hematopoietic+stem+cell+transplantation.">Multicenter study of banked third-party virus-specific T cells to treat severe viral infections after hematopoietic stem cell transplantation.</a> Blood. 121 (26), 5113-5123 (2013).</li></ol>

Both MD Anderson Cancer Center and Dr. Cooper have a financial interest in ZIOPHARM Oncology, Inc., and Intrexon Corporation. On May 7, 2015, Dr. Cooper was appointed as the Chief Executive Officer at ZIOPHARM Oncology.&#160; Dr. Cooper is now a Visiting Scientist at MD Anderson. Dr. Cooper founded and owns InCellerate, Inc. He has patents with Sangamo BioSciences with artificial nucleases. He consults with Targazyme, Inc. (formerly American Stem cells, Inc.), GE Healthcare, Ferring Pharmaceuticals, Fate Therapeutics, Janssen Pharmaceuticals, and Bristol-Myers Squibb. He is on the Scientific Advisory Board of Cellectis. He receives honoraria from Miltenyi Biotec.

Adoptive T-cell therapy has emerged as a viable option to treat B-cell malignancies4. Its therapeutic potential is dependent on infusing the desired number of target antigen specific T cells that lack replicative senescence2. This can be achieved by sorting out a pure population of antigen specific T cells from expanded T cells in compliance with current good manufacturing practices. Two sorting procedures are widely used, namely, fluorescence-activated cell sorting (FACS) and magnetic activated cel...

Hematopoietic stem-cell transplantation (HSCT) 1 can be combined with adoptive T-cell therapy to improve graft-versus-tumor effect and to provide immunity to opportunistic infections2. Generation of antigen-specific donor-derived T cells for infusion has historically required skilled personnel and use of specialized facilities that are GMP-compliant. The delivery of such T cells has resulted in resolution of opportunistic infections3 as well as treating the underlying malignancy4. Recently, investigators have demonstrated that the adoptive transfer of only few thousand virus-specific T cells (~ 1 x 104 &#8211;&#160; 2.5 x 105 cells/kg recipient body weight) can successfully treat opportunistic CMV infections after allogeneic HSCT5-9. A limited number of GMP facilities with associated skilled manufacturing requirements and the high cost associated with cell production has, however, restricted patient access to promising T-cell therapies10. One approach to isolating antigen-specific T cells is based on the CCS using a bi-specific reagent to recognize CD45 and IFN-&#947;. As is shown, this methodology can be used to generate clinical-grade CMV-specific T cells employing an automated cell enrichment CCS device (Figure 1B).
CMV-specific T cells are generated by incubating overlapping peptides from CMV pp65 antigen with leukapheresis total nuclear cells (TNC) from CMV-seropositive donors. These peptides, displayed in the context of human leukocyte antigen (HLA), activate the CMV pp65-specific T cells within the TNC to secrete IFN-&#947;. These T cells can then be &#8220;captured&#8221; and magnetically separated. The operation of the first-generation cell enrichment device (Figure 1A) required personnel skilled in cell culture under GMP conditions, and coordination of staff to undertake the multiple steps necessary to generate a &#8220;captured&#8221; product.
The procedure typically required 10 to 12 hr of continuous operation, and therefore personnel likely need to work over two shifts in the GMP facility. These constraints are now obviated by the implementation of a second-generation device (shown in Figure 1B). This device undertakes magnetic enrichment, similar to the first generation device, but automates other aspects of the CCS in an unbreached approach. This significantly reduces the burden on the GMP team as most of the steps can be accomplished unattended by staff. Furthermore, since the device operates as a closed system, the antigen-specific T cells can be captured and processed on the benchtop except the steps involved in leukapheresis isolation and preparation of materials before starting the instrument. Details of the complete instrumentation and functionality of this second-generation cell enrichment device have been published11.
Here, we describe the steps to enrich CMV pp65-specific T cells from a steady-state apheresis product using the automated cell enrichment CCS system. Once isolated, these CMV-specific T cells may be immediately infused into a patient.

<table border="0" cellpadding="0" cellspacing="0">
	<tbody>
		<tr>
			<td>CliniMACS PBS/EDTA Buffer 3 L bag</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>700-29</td>
			<td></td>
		</tr>
		<tr>
			<td>CliniMACS Prodigy Tubing Set TS 500</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>130-097-182</td>
			<td></td>
		</tr>
		<tr>
			<td>5 L waste bag</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>110-004-067</td>
			<td></td>
		</tr>
		<tr>
			<td>CliniMACS Cytokine Capture System (IFN-gamma)</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>279-01</td>
			<td></td>
		</tr>
		<tr>
			<td>Albumin (Human) 25%&#160;</td>
			<td>Grifols</td>
			<td>58516-5216-2</td>
			<td></td>
		</tr>
		<tr>
			<td>Luer/Spike Interconnector</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>130-018-701</td>
			<td></td>
		</tr>
		<tr>
			<td>0.9 % NaCl Solution (1 L)</td>
			<td>Miltenyi Biotec GmbH</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>MACS GMP PepTivator HCMV pp65</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>170-076-109</td>
			<td></td>
		</tr>
		<tr>
			<td>Water for injections</td>
			<td>Hospira, inc, Lake Forest, IL</td>
			<td>NDC-0409-4887-10</td>
			<td></td>
		</tr>
		<tr>
			<td>MILLEX GV Filter Unit 0.22 &#956;m&#160;</td>
			<td>Millipore</td>
			<td>SLGV033RB</td>
			<td></td>
		</tr>
		<tr>
			<td>TexMACS GMP Medium 2 L bag</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>170-076-306</td>
			<td></td>
		</tr>
		<tr>
			<td>Transfer Bag, 150 mL (for cellular starting material)</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>130-018-301</td>
			<td></td>
		</tr>
		<tr>
			<td>CryoMACS Freezing Bag 50</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>200-074-400</td>
			<td></td>
		</tr>
		<tr>
			<td>60 mL Syringes, sterile</td>
			<td>BD, Laagstraat, Temse, Belgium</td>
			<td>309653</td>
			<td></td>
		</tr>
		<tr>
			<td>CMV sero positive apheresis product</td>
			<td>Key Biologics, LLC, Memphis</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td></td>
			<td></td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Flow Cytometry Materials</td>
			<td>Manufacturer</td>
			<td>Catalog number</td>
			<td></td>
		</tr>
		<tr>
			<td>AB Serum, GemCell</td>
			<td>Gemini Bio-Products, West Sacramento, USA</td>
			<td>100-512</td>
			<td></td>
		</tr>
		<tr>
			<td>CD3-FITC</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>130-080-401</td>
			<td></td>
		</tr>
		<tr>
			<td>CD4-APC</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>130-098-033</td>
			<td></td>
		</tr>
		<tr>
			<td>CD8-APC-Vio770</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>130-098-065</td>
			<td></td>
		</tr>
		<tr>
			<td>CD14-PerCP</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>130-098-072</td>
			<td></td>
		</tr>
		<tr>
			<td>CD20-PerCP</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>130-098-077</td>
			<td></td>
		</tr>
		<tr>
			<td>CD45-VioBlue</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>130-098-136</td>
			<td></td>
		</tr>
		<tr>
			<td>aIFN-&#947;-PE, human</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>130-097-940</td>
			<td></td>
		</tr>
		<tr>
			<td>CD3-PE</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>130-091-374</td>
			<td></td>
		</tr>
		<tr>
			<td>Propidium Iodide Solution (100 &#181;g/mL)</td>
			<td>Miltenyi Biotec GmbH</td>
			<td>130-093-233</td>
			<td></td>
		</tr>
		<tr>
			<td></td>
			<td></td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Equipment</td>
			<td>Manufacturer</td>
			<td>Catalog Number</td>
			<td></td>
		</tr>
		<tr>
			<td>CliniMACS Prodigy Device&#160;</td>
			<td rowspan="2">Miltenyi Biotec GmbH</td>
			<td rowspan="2">200-075-301</td>
			<td></td>
		</tr>
		<tr>
			<td>Software V1.0.0.RC</td>
			<td></td>
		</tr>
		<tr>
			<td>MACSQuant Analyzer 10</td>
			<td rowspan="2">Miltenyi Biotec GmbH</td>
			<td rowspan="2">130-096-343</td>
			<td></td>
		</tr>
		<tr>
			<td>Software 2.4</td>
			<td></td>
		</tr>
		<tr>
			<td>Centrifuge 5415R&#160;</td>
			<td>Eppendorf AG</td>
			<td>22331</td>
			<td></td>
		</tr>
		<tr>
			<td>Cellometer K2</td>
			<td>Nexelom Bioscience, Lawrence, MA</td>
			<td>LB-001-0016</td>
			<td></td>
		</tr>
		<tr>
			<td>Sterile tubing welder SCDIIB</td>
			<td>Terumo Medical Corp., Elkton, MA</td>
			<td>7811</td>
			<td></td>
		</tr>
	</tbody>
</table>

automated cell enrichment of cytomegalovirus-specific t cells for clinical applications using the cytokine-capture system

The adoptive transfer of pathogen-specific T cells can be used to prevent and treat opportunistic infections such as cytomegalovirus (CMV) infection occurring after allogeneic hematopoietic stem-cell transplantation. Viral-specific T cells from allogeneic donors, including third party donors, can be propagated ex vivo in compliance with current good manufacturing practice (cGMP), employing repeated rounds of antigen-driven stimulation to selectively propagate desired T cells. The identification and isolation of antigen-specific T cells can also be undertaken based upon the cytokine capture system of T cells that have been activated to secrete gamma-interferon (IFN-&#947;). However, widespread human application of the cytokine capture system (CCS) to help restore immunity has been limited as the production process is time-consuming and requires a skilled operator. The development of a second-generation cell enrichment device such as CliniMACS Prodigy now enables investigators to generate viral-specific T cells using an automated, less labor-intensive system. This device separates magnetically labeled cells from unlabeled cells using magnetic activated cell sorting technology to generate clinical-grade products, is engineered as a closed system and can be accessed and operated on the benchtop. We demonstrate the operation of this new automated cell enrichment device to manufacture CMV pp65-specific T cells obtained from a steady-state apheresis product obtained from a CMV seropositive donor. These isolated T cells can then be directly infused into a patient under institutional and federal regulatory supervision. All the bio-processing steps including removal of red blood cells, stimulation of T cells, separation of antigen-specific T cells, purification, and washing are fully automated. Devices such as this raise the possibility that T cells for human application can be manufactured outside of dedicated good manufacturing practice (GMP) facilities and instead be produced in blood banking facilities where staff can supervise automated protocols to produce multiple products.

In this study, an automated cell enrichment CCS System was used for automated production of CMV pp65-specific T cells. CMV-specific T cells were enriched from three apheresis cell products. The steady-state apheresis product was harvested over 2 hr from a CMV-seropositive donor and generated 1010 total nuclear cells (TNC). 109 TNC were then activated with CMV pp65-derived peptides (60 nmol) for 4 hr and the IFN-&#947; secreting T cells were isolated using the CCS on the automated cell enrichment dev...

Watch this Scientific Journal Video about Automated Cell Enrichment of Cytomegalovirus-specific T cells for Clinical Applications using the Cytokine-capture System at JoVE.com

Automated Cell Enrichment of Cytomegalovirus-specific T cells for Clinical Applications using the Cytokine-capture System

The goal of this protocol is to manufacture pathogen-specific clinical-grade T cells using a bench-top, automated, second generation cell enrichment device that incorporates a closed cytokine capture system and does not require dedicated staff or use of a GMP facility. The cytomegalovirus pp65-specific-T cells generated can be directly administered to patients.

The adoptive transfer of pathogen-specific T cells can be used to prevent and treat opportunistic infections such as cytomegalovirus (CMV) infection ...

automated-cell-enrichment-cytomegalovirus-specific-t-cells-for

Research

JoVE Journal

Immunology and Infection

12.3K Görüntüleme.  U.T. MD Anderson Cancer Center. The goal of this protocol is to manufacture pathogen-specific clinical-grade T cells using a bench-top, automated, second generation cell enrichment device that incorporates a closed cytokine capture system and does not require dedicated staff or use of a GMP facility. The cytomegalovirus pp65-specific-T cells generated can be directly administered to patients.

Video: Automated Cell Enrichment of Cytomegalovirus-specific T cells for Clinical Applications using the Cytokine-capture System

Retroviral Transduction of T-cell Receptors in Mouse T-cells

T-cell receptors (TCRs) play a central role in the immune system. TCRs on T-cell surfaces can specifically recognize peptide antigens presented by antigen presenting cells (APCs)1. This recognition leads to the activation of T-cells and a series of functional outcomes (e.g. cytokine production, killing of the target cells). Understanding the functional role of TCRs is critical to harness the power of the immune system to treat a variety of immunology related diseases (e.g. cancer or autoimmunity).
It is convenient to study TCRs in mouse models, which can be accomplished in several ways. Making TCR transgenic mouse models is costly and time-consuming and currently there are only a limited number of them available2-4. Alternatively, mice with antigen-specific T-cells can be generated by bone marrow chimera. This method also takes several weeks and requires expertise5. Retroviral transduction of TCRs into in vitro activated mouse T-cells is a quick and relatively easy method to obtain T-cells of desired peptide-MHC specificity. Antigen-specific T-cells can be generated in one week and used in any downstream applications. Studying transduced T-cells also has direct application to human immunotherapy, as adoptive transfer of human T-cells transduced with antigen-specific TCRs is an emerging strategy for cancer treatment6.
Here we present a protocol to retrovirally transduce TCRs into in vitro activated mouse T-cells. Both human and mouse TCR genes can be used. Retroviruses carrying specific TCR genes are generated and used to infect mouse T-cells activated with anti-CD3 and anti-CD28 antibodies. After in vitro expansion, transduced T-cells are analyzed by flow cytometry.

We present a protocol to produce antigen-specific mouse T-cells using retroviral transduction

T-cell receptors (TCRs) play a central role in the immune system. TCRs on T-cell surfaces can specifically recognize peptide antigens presented by antigen ...

Following Cell-fate in E. coli After Infection by Phage Lambda

The system comprising bacteriophage (phage) lambda and the bacterium E. coli has long served as a paradigm for cell-fate determination1,2. Following the simultaneous infection of the cell by a number of phages, one of two pathways is chosen: lytic (virulent) or lysogenic (dormant)3,4. We recently developed a method for fluorescently labeling individual phages, and were able to examine the post-infection decision in real-time under the microscope, at the level of individual phages and cells5. Here, we describe the full procedure for performing the infection experiments described in our earlier work5. This includes the creation of fluorescent phages, infection of the cells, imaging under the microscope and data analysis. The fluorescent phage is a "hybrid", co-expressing wild- type and YFP-fusion versions of the capsid gpD protein. A crude phage lysate is first obtained by inducing a lysogen of the gpD-EYFP (Enhanced Yellow Fluorescent Protein) phage, harboring a plasmid expressing wild type gpD. A series of purification steps are then performed, followed by DAPI-labeling and imaging under the microscope. This is done in order to verify the uniformity, DNA packaging efficiency, fluorescence signal and structural stability of the phage stock. The initial adsorption of phages to bacteria is performed on ice, then followed by a short incubation at 35&deg;C to trigger viral DNA injection6. The phage/bacteria mixture is then moved to the surface of a thin nutrient agar slab, covered with a coverslip and imaged under an epifluorescence microscope. The post-infection process is followed for 4 hr, at 10 min interval. Multiple stage positions are tracked such that ~100 cell infections can be traced in a single experiment. At each position and time point, images are acquired in the phase-contrast and red and green fluorescent channels. The phase-contrast image is used later for automated cell recognition while the fluorescent channels are used to characterize the infection outcome: production of new fluorescent phages (green) followed by cell lysis, or expression of lysogeny factors (red) followed by resumed cell growth and division. The acquired time-lapse movies are processed using a combination of manual and automated methods. Data analysis results in the identification of infection parameters for each infection event (e.g. number and positions of infecting phages) as well as infection outcome (lysis/lysogeny). Additional parameters can be extracted if desired.

Following Cell-fate in E. coli After Infection by Phage Lambda

This article describes the procedure for preparing a fluorescently-labeled version of bacteriophage lambda, infection of E. coli bacteria, following the infection outcome under the microscope, and analysis of infection results.

The system comprising bacteriophage (phage) lambda and the bacterium E. coli has long served as a paradigm for cell-fate determination1,2. Following the ...

piggyBac Transposon System Modification of Primary Human T Cells

The piggyBac transposon system is naturally active, originally derived from the cabbage looper moth1,2. This non-viral system is plasmid based, most commonly utilizing two plasmids with one expressing the piggyBac transposase enzyme and a transposon plasmid harboring the gene(s) of interest between inverted repeat elements which are required for gene transfer activity. PiggyBac mediates gene transfer through a "cut and paste" mechanism whereby the transposase integrates the transposon segment into the genome of the target cell(s) of interest. PiggyBac has demonstrated efficient gene delivery activity in a wide variety of insect1,2, mammalian3-5, and human cells6 including primary human T cells7,8. Recently, a hyperactive piggyBac transposase was generated improving gene transfer efficiency9,10.
Human T lymphocytes are of clinical interest for adoptive immunotherapy of cancer11. Of note, the first clinical trial involving transposon modification of human T cells using the Sleeping beauty transposon system has been approved12. We have previously evaluated the utility of piggyBac as a non-viral methodology for genetic modification of human T cells. We found piggyBac to be efficient in genetic modification of human T cells with a reporter gene and a non-immunogenic inducible suicide gene7. Analysis of genomic integration sites revealed a lack of preference for integration into or near known proto-oncogenes13. We used piggyBac to gene-modify cytotoxic T lymphocytes to carry a chimeric antigen receptor directed against the tumor antigen HER2, and found that gene-modified T cells mediated targeted killing of HER2-positive tumor cells in vitro and in vivo in an orthotopic mouse model14. We have also used piggyBac to generate human T cells resistant to rapamycin, which should be useful in cancer therapies where rapamycin is utilized15.
Herein, we describe a method for using piggyBac to genetically modify primary human T cells. This includes isolation of peripheral blood mononuclear cells (PBMCs) from human blood followed by culture, gene modification, and activation of T cells. For the purpose of this report, T cells were modified with a reporter gene (eGFP) for analysis and quantification of gene expression by flow cytometry.
PiggyBac can be used to modify human T cells with a variety of genes of interest. Although we have used piggyBac to direct T cells to tumor antigens14, we have also used piggyBac to add an inducible safety switch in order to eliminate gene modified cells if needed7. The large cargo capacity of piggyBac has also enabled gene transfer of a large rapamycin resistant mTOR molecule (15 kb)15. Therefore, we present a non-viral methodology for stable gene-modification of primary human T cells for a wide variety of purposes.

piggyBac Transposon System Modification of Primary Human T Cells

We describe a method to genetically modify primary human T cells with a transgene using the non-viral piggyBac transposon system. T cells modified to using the piggyBac transposon system exhibit stable transgene expression.

The piggyBac transposon system is naturally active, originally derived from the cabbage looper moth1,2. This non-viral system is plasmid based, most ...

Peptide:MHC Tetramer-based Enrichment of Epitope-specific T cells

A basic necessity for researchers studying adaptive immunity with in vivo experimental models is an ability to identify T cells based on their T cell antigen receptor (TCR) specificity. Many indirect methods are available in which a bulk population of T cells is stimulated in vitro with a specific antigen and epitope-specific T cells are identified through the measurement of a functional response such as proliferation, cytokine production, or expression of activation markers1. However, these methods only identify epitope-specific T cells exhibiting one of many possible functions, and they are not sensitive enough to detect epitope-specific T cells at naive precursor frequencies. A popular alternative is the TCR transgenic adoptive transfer model, in which monoclonal T cells from a TCR transgenic mouse are seeded into histocompatible hosts to create a large precursor population of epitope-specific T cells that can be easily tracked with the use of a congenic marker antibody2,3. While powerful, this method suffers from experimental artifacts associated with the unphysiological frequency of T cells with specificity for a single epitope4,5. Moreover, this system cannot be used to investigate the functional heterogeneity of epitope-specific T cell clones within a polyclonal population.
	The ideal way to study adaptive immunity should involve the direct detection of epitope-specific T cells from the endogenous T cell repertoire using a method that distinguishes TCR specificity solely by its binding to cognate peptide:MHC (pMHC) complexes. The use of pMHC tetramers and flow cytometry accomplishes this6, but is limited to the detection of high frequency populations of epitope-specific T cells only found following antigen-induced clonal expansion. In this protocol, we describe a method that coordinates the use of pMHC tetramers and magnetic cell enrichment technology to enable detection of extremely low frequency epitope-specific T cells from mouse lymphoid tissues3,7. With this technique, one can comprehensively track entire epitope-specific populations of endogenous T cells in mice at all stages of the immune response.

This protocol describes the use of peptide:MHC tetramers and magnetic microbeads to isolate low frequency populations of epitope-specific T cells and analyze them by flow cytometry. This method enables the direct study of endogenous T cell populations of interest from in vivo experimental systems.

A  basic necessity for researchers studying adaptive immunity with in vivo experimental models is an  ability to identify T cells based on their T cell ...

Quantitative High-throughput Single-cell Cytotoxicity Assay For T Cells

Cancer immunotherapy can harness the specificity of immune response to target and eliminate tumors. Adoptive cell therapy (ACT) based on the adoptive transfer of T cells genetically modified to express a chimeric antigen receptor (CAR) has shown considerable promise in clinical trials1-4. There are several advantages to using CAR+ T cells for the treatment of cancers including the ability to target non-MHC restricted antigens and to functionalize the T cells for optimal survival, homing and persistence within the host; and finally to induce apoptosis of CAR+ T cells in the event of host toxicity5.
Delineating the optimal functions of CAR+ T cells associated with clinical benefit is essential for designing the next generation of clinical trials. Recent advances in live animal imaging like multiphoton microscopy have revolutionized the study of immune cell function in vivo6,7. While these studies have advanced our understanding of T-cell functions in vivo, T-cell based ACT in clinical trials requires the need to link molecular and functional features of T-cell preparations pre-infusion with clinical efficacy post-infusion, by utilizing in vitro assays monitoring T-cell functions like, cytotoxicity and cytokine secretion. Standard flow-cytometry based assays have been developed that determine the overall functioning of populations of T cells at the single-cell level but these are not suitable for monitoring conjugate formation and lifetimes or the ability of the same cell to kill multiple targets8.
Microfabricated arrays designed in biocompatible polymers like polydimethylsiloxane (PDMS) are a particularly attractive method to spatially confine effectors and targets in small volumes9. In combination with automated time-lapse fluorescence microscopy, thousands of effector-target interactions can be monitored simultaneously by imaging individual wells of a nanowell array. We present here a high-throughput methodology for monitoring T-cell mediated cytotoxicity at the single-cell level that can be broadly applied to studying the cytolytic functionality of T cells.

We describe a single-cell high-throughput assay to measure cytotoxicity of T cells when incubated with tumor target cells. This method employs a dense, elastomeric array of sub-nanoliter wells (~100,000 wells/array) to spatially confine the T cells and target cells at defined ratios and is coupled to fluorescence microscopy to monitor effector-target conjugation and subsequent apoptosis.

Cancer immunotherapy can harness the specificity of  immune response to target and eliminate tumors. Adoptive cell therapy (ACT)  based on the adoptive ...

Clinical Application of Sleeping Beauty and Artificial Antigen Presenting Cells to Genetically Modify T Cells from Peripheral and Umbilical Cord Blood

The potency of clinical-grade T cells can be improved by combining gene therapy with immunotherapy to engineer a biologic product with the potential for superior (i) recognition of tumor-associated antigens (TAAs), (ii) persistence after infusion, (iii) potential for migration to tumor sites, and (iv) ability to recycle effector functions within the tumor microenvironment. Most approaches to genetic manipulation of T cells engineered for human application have used retrovirus and lentivirus for the stable expression of CAR1-3. This approach, although compliant with current good manufacturing practice (GMP), can be expensive as it relies on the manufacture and release of clinical-grade recombinant virus from a limited number of production facilities. The electro-transfer of nonviral plasmids is an appealing alternative to transduction since DNA species can be produced to clinical grade at approximately 1/10th the cost of recombinant GMP-grade virus. To improve the efficiency of integration we adapted Sleeping Beauty (SB) transposon and transposase for human application4-8. Our SB system uses two DNA plasmids that consist of a transposon coding for a gene of interest (e.g. 2nd generation CD19-specific CAR transgene, designated CD19RCD28) and a transposase (e.g. SB11) which inserts the transgene into TA dinucleotide repeats9-11. To generate clinically-sufficient numbers of genetically modified T cells we use K562-derived artificial antigen presenting cells (aAPC) (clone #4) modified to express a TAA (e.g. CD19) as well as the T cell costimulatory molecules CD86, CD137L, a membrane-bound version of interleukin (IL)-15 (peptide fused to modified IgG4 Fc region) and CD64 (Fc-&gamma; receptor 1) for the loading of monoclonal antibodies (mAb)12. In this report, we demonstrate the procedures that can be undertaken in compliance with cGMP to generate CD19-specific CAR+ T cells suitable for human application. This was achieved by the synchronous electro-transfer of two DNA plasmids, a SB transposon (CD19RCD28) and a SB transposase (SB11) followed by retrieval of stable integrants by the every-7-day additions (stimulation cycle) of &gamma;-irradiated aAPC (clone #4) in the presence of soluble recombinant human IL-2 and IL-2113. Typically 4 cycles (28 days of continuous culture) are undertaken to generate clinically-appealing numbers of T cells that stably express the CAR. This methodology to manufacturing clinical-grade CD19-specific T cells can be applied to T cells derived from peripheral blood (PB) or umbilical cord blood (UCB). Furthermore, this approach can be harnessed to generate T cells to diverse tumor types by pairing the specificity of the introduced CAR with expression of the TAA, recognized by the CAR, on the aAPC.

Clinical Application of Sleeping Beauty and Artificial Antigen Presenting Cells to Genetically Modify T Cells from Peripheral and Umbilical Cord Blood

T cells expressing a CD19-specific chimeric antigen receptor (CAR) are infused as investigational treatment of B-cell malignancies in our first-in-human gene therapy trials. We describe genetic modification of T cells using the Sleeping Beauty (SB) system to introduce CD19-specific CAR and selective propagation on designer CD19+ artificial antigen presenting cells.

The potency of clinical-grade T cells can be improved by combining gene therapy with immunotherapy to engineer  a biologic product with the potential for ...

Monitoring Dendritic Cell Migration using 19F / 1H Magnetic Resonance Imaging

Continuous advancements in noninvasive imaging modalities such as magnetic resonance imaging (MRI) have greatly improved our ability to study physiological or pathological processes in living organisms. MRI is also proving to be a valuable tool for capturing transplanted cells in vivo. Initial cell labeling strategies for MRI made use of contrast agents that influence the MR relaxation times (T1, T2, T2*) and lead to an enhancement (T1) or depletion (T2*) of signal where labeled cells are present. T2* enhancement agents such as ultrasmall iron oxide agents (USPIO) have been employed to study cell migration and some have also been approved by the FDA for clinical application. A drawback of T2* agents is the difficulty to distinguish the signal extinction created by the labeled cells from other artifacts such as blood clots, micro bleeds or air bubbles. In this article, we describe an emerging technique for tracking cells in vivo that is based on labeling the cells with fluorine (19F)-rich particles. These particles are prepared by emulsifying perfluorocarbon (PFC) compounds and then used to label cells, which subsequently can be imaged by 19F MRI. Important advantages of PFCs for cell tracking in vivo include (i) the absence of carbon-bound 19F in vivo, which then yields background-free images and complete cell selectivityand(ii) the possibility to quantify the cell signal by 19F MR spectroscopy.

Monitoring Dendritic Cell Migration using 19F / 1H Magnetic Resonance Imaging

Tracking of cells using MRI has gained remarkable attention in the past years. This protocol describes the labeling of dendritic cells with fluorine (19F)-rich particles, the in vivo application of these cells, and monitoring the extent of their migration to the draining lymph node with 19F/1H MRI and 19F MRS.

Continuous  advancements in noninvasive imaging modalities such as magnetic resonance  imaging (MRI) have greatly improved our ability to study ...

Assessing the Innate Sensing of HIV-1 Infected CD4+ T Cells by Plasmacytoid Dendritic Cells Using an Ex vivo Co-culture System.

HIV-1 innate sensing requires direct contact of infected CD4+ T cells with plasmacytoid dendritic cells (pDCs). In order to study this process, the protocols described here use freshly isolated human peripheral blood mononuclear cells (PBMCs) or plasmacytoid dendritic cells (pDCs) to sense infections in either T cell line (MT4) or heterologous primary CD4+ T cells. In order to ensure proper sensing, it is essential that PBMC are isolated immediately after blood collection and that optimal percentage of infected T cells are used. Furthermore, multi-parametric flow cytometric staining can be used to confirm that PBMC samples contain the different cell lineages at physiological ratios. A number of controls can also be included to evaluate viability and functionality of pDCs. These include, the presence of specific surface markers, assessing cellular responses to known agonist of Toll-Like Receptors (TLR) pathways, and confirming a lack of spontaneous type-I interferon (IFN) production. In this system, freshly isolated PBMCs or pDCs are co-cultured with HIV-1 infected cells in 96 well plates for 18-22 hr. Supernatants from these co-cultures are then used to determine the levels of bioactive type-I IFNs by monitoring the activation of the ISGF3 pathway in HEK-Blue IFN-&#945;/&#946; cells. Prior and during co-culture conditions, target cells can be subjected to flow cytometric analysis to determine a number of parameters, including the percentage of infected cells, levels of specific surface markers, and differential killing of infected cells. Although, these protocols were initially developed to follow type-I IFN production, they could potentially be used to study other imuno-modulatory molecules released from pDCs and to gain further insight into the molecular mechanisms governing HIV-1 innate sensing.

Assessing the Innate Sensing of HIV-1 Infected CD4+ T Cells by Plasmacytoid Dendritic Cells Using an Ex vivo Co-culture System.

Unlike cell-free HIV-1 particles, infected CD4+ T cells are effectively sensed by plasmacytoid dendritic cells (pDCs). This manuscript describes a method where peripheral blood mononuclear cells (PBMCs) or isolated pDCs are co-cultured with HIV-1 infected T cells to evaluate innate sensing by pDCs as assessed by release of type-I IFN.

HIV-1 innate sensing requires direct contact of infected CD4+ T cells with plasmacytoid dendritic cells (pDCs). In order to study this process, the ...

Mouse Na&#239;ve CD4+ T Cell Isolation and In vitro Differentiation into T Cell Subsets

Antigen inexperienced (na&#239;ve) CD4+ T cells undergo expansion and differentiation to effector subsets at the time of T cell receptor (TCR) recognition of cognate antigen presented on MHC class II. The cytokine signals present in the environment at the time of TCR activation are a major factor in determining the effector fate of a na&#239;ve CD4+ T cell. Although the cytokine environment during na&#239;ve T cell activation may be complex and involve both redundant and opposing signals in vivo, the addition of various cytokine combinations during naive CD4+ T cell activation in vitro can readily promote the establishment of effector T helper lineages with hallmark cytokine and transcription factor expression. Such differentiation experiments are commonly used as a first step for the evaluation of targets believed to promote or inhibit the development of certain CD4+ T helper subsets. The addition of mediators, such as signaling agonists, antagonists, or other cytokines, during the differentiation process can also be used to study the influence of a particular target on T cell differentiation. Here, we describe a basic protocol for the isolation of na&#239;ve T cells from mouse and the subsequent steps necessary for polarizing na&#239;ve cells to various T helper effector lineages in vitro.

Mouse Na&amp;#239;ve CD4+ T Cell Isolation and In vitro Differentiation into T Cell Subsets

Na&#239;ve CD4+ T cells polarize to various subsets depending on the environment at the time of activation. The differentiation of na&#239;ve CD4+ T cells to various effector subsets can be achieved in vitro through the addition of T cell receptor stimuli and specific cytokine signals.

Antigen inexperienced (na&#239;ve) CD4+ T cells undergo expansion and differentiation to effector subsets at the time of T cell receptor (TCR) recognition ...

Development of Stem Cell-derived Antigen-specific Regulatory T Cells Against Autoimmunity

Autoimmune diseases arise due to the loss of immunological self-tolerance. Regulatory T cells (Tregs) are important mediators of immunologic self-tolerance. Tregs represent about 5 - 10% of the mature CD4+ T cell subpopulation in mice and humans, with about 1 - 2% of those Tregs circulating in the peripheral blood. Induced pluripotent stem cells (iPSCs) can be differentiated into functional Tregs, which have a potential to be used for cell-based therapies of autoimmune diseases. Here, we present a method to develop antigen (Ag)-specific Tregs from iPSCs (i.e., iPSC-Tregs). The method is based on incorporating the transcription factor FoxP3 and an Ag-specific T cell receptor (TCR) into iPSCs and then differentiating on OP9 stromal cells expressing Notch ligands delta-like (DL) 1 and DL4. Following in vitro differentiation, the iPSC-Tregs express CD4, CD8, CD3, CD25, FoxP3, and Ag-specific TCR and are able to respond to Ag stimulation. This method has been successfully applied to cell-based therapy of autoimmune arthritis in a murine model. Adoptive transfer of these Ag-specific iPSC-Tregs into Ag-induced arthritis (AIA)-bearing mice has the ability to reduce joint inflammation and swelling and to prevent bone loss.

We present here a method to develop functional antigen (Ag)-specific regulatory T cells (Tregs) from induced pluripotent stem cells (iPSCs) for immunotherapy of autoimmune arthritis in a murine model.