The authors would like to acknowledge the technical contribution of Gloria A Benavides. This work was supported by American Heart Association 13PRE16390001 (SR), NIH T32HL07918 (PAK), NIH T32HL007457 (TM), P30DK056336 (BKC), NIDDK Diabetic Complications Consortium (DiaComp, www.diacomp.org) grant DK076169 (subaward VDU), and the O&#8217;Brien Center P30 DK079337 (VDU).

All protocols described in this manuscript for blood collection, isolation and analysis have been reviewed and approved by the Institutional Review Board at the University of Alabama at Birmingham.
1. Cell Isolation (Modified from Histopaque Sigma-Aldrich Protocol No. 1119 and Miltenyi Biotec MicroBead Positive and Negative Selection Protocols)
<ol>
	<li>Centrifuge whole blood (collected in ACD or EDTA tubes) at 500 x g for 15 min&#160;in a centrifuge with a swinging-bucket rotor (acceleration = 5-6, and no brake).</li>
	<li>Remove the top layer that contains the platelet rich plasma (PRP) with a transfer pipette until 1 cm remains above the cell layer (erythrocyte/buffy coat). Set aside the PRP at room temperature for processing later.</li>
	<li>Transfer the buffy coat to a sterile 50 ml conical tube, dilute to 24 ml with basal RPMI or to at least 4x the starting buffy coat volume. 
	Note: The upper half of the RBC layer may have to be included although this will result in increasing the RPMI volume proportionally.</li>
	<li>Prepare the density gradient using low density Ficoll with a specific gravity of 1.077 (1077) for the top layer and high density Ficoll with a specific gravity of 1.119 (1119) for the bottom layer in three 15 ml conical tubes (3 ml each). To perform this step, first add 1077 to each tube. Using a 5 ml narrow pipette add 1119 to the bottom of the tube by placing the pipette tip beneath 1077 and slowly release the reagent without mixing with the upper gradient. A total of 6 ml of density gradient media should be present at this stage with a visible phase of separation at the 3 ml mark.</li>
	<li>Using an automated pipette, add 8 ml of diluted blood (from step 1.3) gently to each gradient tube using the low-power setting to prevent from disturbing the gradient layers. The total volume should be 14 ml at this step.</li>
	<li>Centrifuge tubes at 700 x g for 30 min at room temperature (acceleration 6, no brake). 
	Note: At this stage, three distinct cell bands should be evident (Figure 1A). The uppermost bands (between 1077 and plasma) contains mononuclear cells (MNCs) and platelets, and the middle band (between 1007 and 1119) contains polymorphonuclear cells (PMNs) and lower band (below 1119) contains RBCs.</li>
	<li>Collect the MNC and PMN separately by using sterile glass pipettes without disturbing the other cell bands. Combine the MNC population from each tube into a sterile 50 ml conical tube. Repeat this for the PMN population as well.</li>
	<li>Add 4 volumes of RPMI to each tube containing the MNC and PMN fractions respectively to dilute the density gradient.</li>
	<li>Centrifuge tubes at 700 x g for 10 min at room temperature.</li>
	<li>Resuspend MNC cell pellet and PMN cell pellet in 1 ml RPMI containing 0.5% ultra-pure fatty acid-free BSA (RPMI-BSA) and transfer to sterile 1.5 ml tubes.&#160;Pellet the cells using a benchtop picofuge for 30 sec.</li>
	<li>Discard the supernatant and resuspend each cell pellet in 80 &#181;l RPMI-BSA.</li>
	<li>Add 20 &#181;l of magnetic bead labeled-antiCD14 antibody to the tube containing the MNC fraction for positive selection of monocytes.&#160;For the tube containing the PMN cell fraction, add 20 &#181;l of magnetic bead labeled-antiCD15 antibody for positive selection of neutrophils.&#160;Incubate each cell suspension for 15 min at 4 &#186;C.</li>
	<li>Wash each cell suspension with 1 ml RPMI-BSA media and pellet as before and resuspend each pellet in 500 &#181;l RPMI-BSA.</li>
	<li>The labeled cells are separated in the magnetic field of the magnetic activated cell sorting (MACS) separator. Prepare the MACS LS columns (one for each cell suspension) by placing the column on the MACS separator and washing with 3 ml of RPMI-BSA prior to adding the cell suspension.</li>
	<li>After applying cell suspensions, wash each column 3x with 3 ml of RPMI-BSA media (make sure to let the media drain completely between washes). Collect the cell suspension flow-through and column washes into a sterile tube.</li>
	<li>To isolate monocytes and neutrophils, remove the column from the magnetic field after the final wash and elute the positively selected cells into a sterile tube with 5 ml of RPMI-BSA using the column plunger.</li>
	<li>To isolate lymphocytes pellet the flow-through-wash fraction of the MNCs from step 1.15 at 300 x g for 10 min.&#160;Discard the supernatant and resuspend the cell pellet in 80 &#181;l&#160;RPMI-BSA. Add 20 &#181;l of CD61 and CD235a antibodies and incubate cell suspension for 15 min&#160;at 4 &#186;C.&#160;Repeat the MACS separation as before and collect the flow though containing the lymphocytes.</li>
	<li>To pellet monocytes, neutrophils, and lymphocytes fractions, centrifuge as before (step 1.9) and discard supernatants.&#160;Cell pellets should be resuspended in 1 ml extracellular flux media (XF-DMEM) for counting. 
	Note: 8 ml of whole blood should result in 1-5 x 106 monocytes/ml, and 5-20 x 106 lymphocytes and neutrophils/ml.</li>
	<li>To isolate platelets, centrifuge PRP (step 1.2) for 8-10 min at 1,500 x g at room temperature. Remove the plasma and wash cell pellet once with sterile 5 ml PBS supplemented with 1 &#181;g/ml PGI2, repellet and suspend final pellet in 1 ml of PBS-PGI2 buffer.</li>
	<li>Determine platelet count by turbidimetry once the platelets are suspended in PBS-PGI2 buffer by spectrophotometer as described by Walkowiak et al. using the following equation: [6.23/(2.016 &#8211; Abs800)] &#8211; 3.09 x dilution factor = # x 108&#160;platelets/ml&#160;12.</li>
</ol>
2. Plating of the Cells
<ol>
	<li>Preparation of Cell-Tak (cell adhesive):&#160; Add 90 &#181;l cell adhesive to 180 &#181;l diH20, 540 &#181;l of 0.1 N sodium bicarbonate (pH 8.0), and adjust pH to 7.2-7.8 using 1 N NaOH. Prepare XF plates (24-well, V7 microplates) by coating each well with 30 &#181;l of prepared cell adhesive. 
	Note:&#160; The cell adhesive should be prepared fresh for each use.</li>
	<li>Incubate plate at 37 &#186;C for 20-30 min then aspirate cell adhesive and wash wells with PBS twice (1 ml/well).</li>
	<li>Perform a cell count on isolated monocytes, lymphocytes, neutrophils and platelets and bring to appropriate volume using XF-DMEM to allow a seeding density of 250k&#160;cells/well for monocytes, lymphocytes, and neutrophils, and 25 x 106/well for platelets. Alternatively, to measure oxidative burst response, neutrophils can be seeded at 125k&#160;cells/well. The final seeding volume for each cell suspension should be 200 &#181;l/well.</li>
	<li>Centrifuge the plate at 200 x g for 1 sec with no brake. Rotate the plate 180&#730; and centrifuge again with no brake at 300 x g.</li>
	<li>Bring final well volume to 660 &#181;l with XF-DMEM and incubate at 37 &#186;C for 30 min prior to XF assay. Note: Photomicrographs of plated cells before and after the assay can be used to ensure adequate plating and rule out cell detachment.</li>
</ol>
3. Preparation of a 24-well Extracellular Flux Assay Plate (XF24)
<ol>
	<li>Hydrate XF probes with calibrant solution for a minimum of 2 hr prior to assay.</li>
	<li>Prepare 10x stocks of 0.5 &#181;g/ml oligomycin, 0.6 &#181;M FCCP, and 10 &#181;M antimycin A in XF-DMEM and load 75 &#181;l of stock solutions into cartridge injection ports in the above order. If oxidative burst measurements are to be obtained, injection of 10x stock of 100 ng/ml PMA can be injected after antimycin-A.</li>
	<li>Calibrate the hydrated and loaded cartridge and perform the XF assay. The detailed methods for analysis and interpretation of both oxygen consumption and pH changes have been described in previous publications9,13,14 and are not discussed in detail here.</li>
	<li>After XF assay, aspirate all but the last 50 &#181;l of XF-DMEM after assay to prevent loss of cells from the plate and add 50 &#181;l RIPA cell lysis buffer and perform a protein assay for normalization.</li>
</ol>

<ol>
	<li>Mancuso, 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=Mitochondria,+cognitive+impairment,+and+Alzheimer's+disease.">Mitochondria, cognitive impairment, and Alzheimer's disease.</a> Int. J. Alzheimer's Dis. 2009, (2009).</li><li>Jin, S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Autophagy,+mitochondrial+quality+control,+and+oncogenesis.">Autophagy, mitochondrial quality control, and oncogenesis.</a> Autophagy. 2, 80-84 (2006).</li><li>Cordero, M. D., 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=Mitochondrial+dysfunction+and+mitophagy+activation+in+blood+mononuclear+cells+of+fibromyalgia+patients:+implications+in+the+pathogenesis+of+the+disease.">Mitochondrial dysfunction and mitophagy activation in blood mononuclear cells of fibromyalgia patients: implications in the pathogenesis of the disease.</a> Arthritis Res. Ther. 12, R17 (2010).</li><li>Japiassu, 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=Bioenergetic+failure+of+human+peripheral+blood+monocytes+in+patients+with+septic+shock+is+mediated+by+reduced+F1Fo+adenosine-5'-triphosphate+synthase+activity.">Bioenergetic failure of human peripheral blood monocytes in patients with septic shock is mediated by reduced F1Fo adenosine-5'-triphosphate synthase activity.</a> Crit. Med. 39, 1056-1063 (2011).</li><li>Widlansky, M. E., 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=Altered+mitochondrial+membrane+potential,+mass,+and+morphology+in+the+mononuclear+cells+of+humans+with+type+2+diabetes.">Altered mitochondrial membrane potential, mass, and morphology in the mononuclear cells of humans with type 2 diabetes.</a> Transl. Res. 156, 15-25 (2010).</li><li>Shi, 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=Effects+of+ageing+and+Alzheimer's+disease+on+mitochondrial+function+of+human+platelets.">Effects of ageing and Alzheimer's disease on mitochondrial function of human platelets.</a> Exp. Gerontol. 43, 589-594 (2008).</li><li>Avila, 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=Platelet+mitochondrial+dysfunction+is+evident+in+type+2+diabetes+in+association+with+modifications+of+mitochondrial+anti-oxidant+stress+proteins.">Platelet mitochondrial dysfunction is evident in type 2 diabetes in association with modifications of mitochondrial anti-oxidant stress proteins.</a> Exp. Clin. Endocrinol. Diabetes. 120, 248-251 (2012).</li><li>Chacko, B. K., 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=Methods+for+defining+distinct+bioenergetic+profiles+in+platelets,+lymphocytes,+monocytes,+and+neutrophils,+and+the+oxidative+burst+from+human+blood.">Methods for defining distinct bioenergetic profiles in platelets, lymphocytes, monocytes, and neutrophils, and the oxidative burst from human blood.</a> Lab. Invest. 93, 690-700 (2013).</li><li>Hill, B. 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=Integration+of+cellular+bioenergetics+with+mitochondrial+quality+control+and+autophagy.">Integration of cellular bioenergetics with mitochondrial quality control and autophagy.</a> Biol. Chem. 393, 1485-1512 (2012).</li><li>Hultqvist, 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=Enhanced+autoimmunity,+arthritis,+and+encephalomyelitis+in+mice+with+a+reduced+oxidative+burst+due+to+a+mutation+in+the+Ncf1+gene.">Enhanced autoimmunity, arthritis, and encephalomyelitis in mice with a reduced oxidative burst due to a mutation in the Ncf1 gene.</a> Proc. Natl. Acad. Sci. U.S.A. 101, 12646-12651 (2004).</li><li>Rosa-Borges, A., 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=Glucose-6-phosphate+dehydrogenase+deficiency+with+recurrent+infections:+case+report.">Glucose-6-phosphate dehydrogenase deficiency with recurrent infections: case report.</a> J. Ped. 77, 331-336 (2001).</li><li>Walkowiak, B., Kesy, A., Michalec, L. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Microplate+reader--a+convenient+tool+in+studies+of+blood+coagulation.">Microplate reader--a convenient tool in studies of blood coagulation.</a> Thromb. Res. 87, 95-103 (1997).</li><li>Dranka, B. P., 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=Assessing+bioenergetic+function+in+response+to+oxidative+stress+by+metabolic+profiling.">Assessing bioenergetic function in response to oxidative stress by metabolic profiling.</a> Free Radic. Biol. Med. 51, 1621-1635 (2011).</li><li>Nicholls, D. 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=Bioenergetic+profile+experiment+using+C2C12+myoblast+cells.">Bioenergetic profile experiment using C2C12 myoblast cells.</a> J. Vis. Exp.. (46), e2511 (2010).</li></ol>

VDU&#160;is a member of the Seahorse Bioscience&#160;Scientific Advisory Board.

This protocol represents the compilation of several commonly utilized techniques for blood cell isolation in a manner suitable for bioenergetics analysis. The contiguous techniques presented are advantageous to other isolation methods (i.e. FACs analysis) for their ability to isolate large numbers of cells in controlled media conditions with minimal stresses placed on the isolated cells. It has the disadvantage of lengthy isolations even with minimal interruptions. This protocol serves as the basis for the isolation of primary blood cells from human subjects, which can be extrapolated into clinical settings and translational research.
MACS separation is a reliable cell isolation technique that offers the possibility of isolating cells directly from whole blood; however, this method requires greater amounts of antibody and is not optimal for the isolation of all four distinct cell types as described in this method. There has been no evidence to show that the positive selection of leukocytes by MACS separation results in activation using our isolation protocol. MACS columns function by sequestration of labeled cells in a magnetic field using antibodies conjugated to 50 nm superparamagnetic particles. Labeled cells are then eluted off the column. Positive and negative selections are implemented in this protocol to ensure rapid isolation and purity. If inadequate cell numbers are obtained from isolation or purity is in question, more antibodies can be added to the sample as per the vendor&#8217;s instruction and second passage through the LS column may result in greater purity (Table 2). Our laboratory found high purity and plating efficiency using the existing protocol by analyzing final cell suspensions by FACS analysis8.
Extracellular flux analyzers have the ability to monitor both oxygen consumption and media acidification in real time over that of other electrodes. The oxygen consumption as observed by the oxidative burst response in monocytes and neutrophils is NADPH oxidase dependent as shown by inhibition with DPI8. We have seen a time dependent loss in oxidative burst capacity with prolonged isolations or extended XF assays. This protocol was designed and developed for use on the XF24 but is also compatible with the XF96 at approximately a third to one half of the XF24 cell seeding densities (Figure 3).
In design of this protocol, adherence to existing protocols for each technique was required for optimal performance with modifications made solely to control media conditions for bioenergetic analysis. After mastering techniques, such a protocol can be used in a wide array of translational and research applications to measure the toxicity or effectiveness of treatment strategies, explore metabolic characteristics of disease,&#160;and oxidant production by monocyte and neutrophils in inflammatory conditions.

Monitoring the bioenergetic health of immune cells (monocytes, lymphocytes, neutrophils) and platelets from blood has been recognized for some time as a potentially useful diagnostic tool to assess the overall bioenergetic health of an individual. There is an emerging body of literature attributing a number of diseases such as cancer, cardiovascular diseases and neurodegenerative diseases to mitochondrial dysfunction1,2. This is clinically important since mitochondrial dysfunction can initiate a series of cellular events that promote pro-inflammatory signaling pathways or lead to cell death. Several studies have characterized mitochondrial function of peripheral blood mononuclear cells and platelets in conditions such as fibromyalgia, diabetes, septic shock, and Alzheimer&#8217;s disease3-7. For example, a recent study evaluated the bioenergetics of platelets as a marker for mitochondrial function and found that platelets from Type 2 diabetic patients had diminished mitochondrial oxygen consumption7,8. From these findings and others, it is clear that monocytes, lymphocytes, neutrophils, and platelets can serve as surrogate markers of changes in bioenergetics under pathological conditions since they survey the systemic circulation and may reflect local and global metabolic changes. To determine whether this approach has prognostic or diagnostic value a high throughput method of analysis and a consistent method for cell preparation is required.
The methods to measure mitochondrial function in leukocytes and platelets have previously involved isolation of mitochondria or assessment of cellular bioenergetics in intact cells4,9. The advantage of cellular bioenergetic assessment using an extracellular flux (XF) analyzer is that the mitochondrial function in cells can be established with endogenous substrates and respiratory parameters such as proton leak and maximal respiratory capacity can be determined.&#160;We and others have used this technology to show that bioenergetic profiles in platelets, monocytes and lymphocytes isolated from human blood can be established and compared among cell types8. In addition, both neutrophils and monocytes possess an oxidative burst capacity in which NAPDH oxidases are activated and consume oxygen to form superoxide.&#160;Importantly, this pathway is a key component of innate immunity and is modulated by systemic inflammation. For example, it has been shown that changes in the oxidative burst capacity are associated with various autoimmune diseases such as multiple sclerosis, arthritis, and recurrent infections10,11. Currently there are no high throughput quantitative assays available to measure the oxidative burst in clinical samples.&#160;This is important since characterizing the oxidative burst capacity of neutrophils and monocytes may also serve as an important diagnostic tool for several pathologies.
The key technical challenges have been low sensitivity for measurement of oxygen consumption using conventional polarographic techniques and the need to use attached cells when using more sensitive microplate fluorometric techniques.&#160;In this practical video, we describe the technical solution to these problems.&#160;We detail the methods for the isolation, plating and measurement of bioenergetics of monocytes, lymphocytes, neutrophils, and platelets and the oxidative burst of monocytes and neutrophils from human blood. This method is suitable for clinical assessment of bioenergetics and oxidative burst for investigators that have access to a patient population and the capability to obtain fresh blood samples.

<table border="0" cellpadding="0" cellspacing="0" width="860">
	<colgroup>
		<col span="3" />
		<col />
	</colgroup>
	<tbody>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">QuadroMACS Starting Kit incl. QuadroMACS Separator and MACS MultiStand</td>
			<td style="width:215px;">Miltenyi Biotec</td>
			<td style="width:215px;">130-094-833</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;"><a name="RANGE!A3">CD235a (Glycophorin A) MicroBeads, human</a></td>
			<td style="width:215px;">Miltenyi Biotec</td>
			<td style="width:215px;">130-050-501</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">CD61 MicroBeads, human&#160; for platelets</td>
			<td style="width:215px;">Miltenyi Biotec</td>
			<td style="width:215px;">130-051-101</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">CD14 MicroBeads, human&#160; for monocytes</td>
			<td style="width:215px;">Miltenyi Biotec</td>
			<td style="width:215px;">130-050-201</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">CD15 MicroBeads, human&#160; for granulocytes</td>
			<td style="width:215px;">Miltenyi Biotec</td>
			<td style="width:215px;">130-046-601</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">LS Columns</td>
			<td style="width:215px;">Miltenyi Biotec</td>
			<td style="width:215px;">130-042-401</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">BD Vacutainer ACD Blood collection tubes</td>
			<td style="width:215px;">Fisher</td>
			<td style="width:215px;">02-684-26</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">RPMI 1640</td>
			<td style="width:215px;">Gibco</td>
			<td style="width:215px;">11835-030</td>
			<td style="width:215px;">with L-glutamine and without phenol red</td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">Prostaglandin I2, sodium salt</td>
			<td style="width:215px;">Cayman</td>
			<td style="width:215px;">18220</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">1.5 ml semi-micro cuvettes</td>
			<td style="width:215px;">Phenix Research Products</td>
			<td style="width:215px;">SC-2410</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">Histopaque density gradient, specific gravity 1.077</td>
			<td style="width:215px;">Sigma</td>
			<td style="width:215px;">10771</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">Histopaque density gradient, specific gravity 1.119</td>
			<td style="width:215px;">Sigma</td>
			<td style="width:215px;">11191</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">Bovine Serum Albumin Fraction V</td>
			<td style="width:215px;">Roche</td>
			<td style="width:215px;">3117405001</td>
			<td style="width:215px;">fatty-acid ultra-free</td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">Phorbol 12-myristate 13-acetate</td>
			<td style="width:215px;">Sigma</td>
			<td style="width:215px;">P8139</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">XF24 FluxPak</td>
			<td style="width:215px;">Seahorse Biosciences</td>
			<td style="width:215px;">100850-001</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">DMEM</td>
			<td style="width:215px;">Fisher</td>
			<td style="width:215px;">MT90113PB</td>
			<td style="width:215px;">w/o Glucose, L-Glutamine, Pyruvate, Phenol Red, and Bicarbonate</td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">L-Glutamine, 200mM (100x)</td>
			<td style="width:215px;">Invitrogen</td>
			<td style="width:215px;">25030-081</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">D-Glucose</td>
			<td style="width:215px;">Sigma</td>
			<td style="width:215px;">G7528</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">Sodium Pyruvate</td>
			<td style="width:215px;">Sigma</td>
			<td style="width:215px;">P8574</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">Cell-Tak (cell adhesive)</td>
			<td style="width:215px;">BD Biosciences</td>
			<td style="width:215px;">CB-40242</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">Oligomycin</td>
			<td style="width:215px;">Sigma</td>
			<td style="width:215px;">O4876</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">Antimycin A</td>
			<td style="width:215px;">Sigma</td>
			<td style="width:215px;">A8674</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">(FCCP) Carbonyl cyanide 4-(trifluoromethoxy)phenylhydrazone</td>
			<td style="width:215px;">Sigma</td>
			<td style="width:215px;">C-2920</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">DC Protein Assay Reagent A</td>
			<td style="width:215px;">Bio-Rad</td>
			<td style="width:215px;">500-0113</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">DC Protein Assay Reagent S</td>
			<td style="width:215px;">Bio-Rad</td>
			<td style="width:215px;">500-0015</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">DC Protein Assay Reagent B</td>
			<td style="width:215px;">Bio-Rad</td>
			<td style="width:215px;">500-0114</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;"></td>
			<td style="width:215px;"></td>
			<td style="width:215px;"></td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">Equipment</td>
			<td style="width:215px;">Vendor</td>
			<td style="width:215px;">Product #</td>
			<td style="width:215px;">Comments/Description</td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">Seahorse</td>
			<td style="width:215px;">Seahorse Biosciences</td>
			<td style="width:215px;"></td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">QuadroMACS Separator and MACS MultiStand</td>
			<td style="width:215px;">Miltenyi Biotec</td>
			<td style="width:215px;">130-090-976 and 24039</td>
			<td style="width:215px;"></td>
		</tr>
		<tr height="60">
			<td height="60" style="height:60px;width:215px;">Spectrophotometer</td>
			<td style="width:215px;"></td>
			<td style="width:215px;"></td>
			<td style="width:215px;"></td>
		</tr>
	</tbody>
</table>

bioenergetics and the oxidative burst: protocols for the isolation and evaluation of human leukocytes and platelets

Mitochondrial dysfunction is known to play a significant role in a number of pathological conditions such as atherosclerosis, diabetes, septic shock, and neurodegenerative diseases but assessing changes in bioenergetic function in patients is challenging.&#160;Although diseases such as diabetes or atherosclerosis present clinically with specific organ impairment, the systemic components of the pathology, such as hyperglycemia or inflammation, can alter bioenergetic function in circulating leukocytes or platelets. This concept has been recognized for some time but its widespread application has been constrained by the large number of primary cells needed for bioenergetic analysis.&#160;This technical limitation has been overcome by combining the specificity of the magnetic bead isolation techniques, cell adhesion techniques, which allow cells to be attached without activation to microplates, and the sensitivity of new technologies designed for high throughput microplate respirometry.&#160;An example of this equipment is the extracellular flux analyzer. Such instrumentation typically uses oxygen and pH sensitive probes to measure rates of change in these parameters in adherent cells, which can then be related to metabolism. Here we detail the methods for the isolation and plating of monocytes, lymphocytes, neutrophils and platelets, without activation, from human blood and the analysis of mitochondrial bioenergetic function in these cells. In addition, we demonstrate how the oxidative burst in monocytes and neutrophils can also be measured in the same samples. Since these methods use only 8-20 ml human blood they have potential for monitoring reactive oxygen species generation and bioenergetics in a clinical setting.

In order to assess the bioenergetics of blood cells, whole blood is collected from human subjects by venipuncture in an EDTA or ACD vacutainer collection tube. The isolation of leukocytes and platelets following blood collection is visualized in Figure 1A as detailed in the protocol. Whole blood samples are processed within 8 hr of collection to avoid cell death and activation.&#160;Extended storage times greater than 8 hr have not been tested but may result in altered bioenergetics and be less representative of physiological conditions. Acid citrate dextrose (ACD-8 ml) and EDTA vacutainer tubes have been used for cell isolations with no observed effect on the bioenergetic function of isolated cells. Anticoagulants are necessary as clots reduce the number of cells obtained, interfere with proper phase formation during Ficoll gradient centrifugation, and result in little to no platelets obtained in centrifuged serum. All blood represents a biological hazard and proper personal protective equipment must be implemented throughout the entire procedure even after cell populations are isolated or cell lysates are generated. Samples are to be disposed of in accordance with the institution&#8217;s human waste disposal standards.
Whole blood is centrifuged to separate the platelet rich plasma from the buffy coat, the white layer just above the packed red blood cells which contains the leukocytes. The buffy coat is applied to density gradients and centrifuged to obtain the peripheral blood mononuclear cells (monocytes and lymphocytes) and polymorphonuclear cells (granulocytes). RBC contamination of the individual MNC and PMN cell phases is common at this stage and should be resolved during the MACS purification. The various cell types are then obtained by incubation with magnetic antibodies to obtain pure fractions. Monocytes are collected by incubation of the PBMC fraction with CD14, the flow-through from the monocytes contain lymphocytes, which are then depleted of RBCs and platelets. The neutrophils are obtained by incubation of the polymorphonuclear cell layer with CD15 antibody (Figure 1A). Thereafter, the platelets can be pelleted by centrifugation of the platelet rich plasma and washed to remove other plasma components. After these selections the platelets, CD14+ monocytes, lymphocytes, CD15+ neutrophils can be counted and plated on a cell adhesion medium-coated XF analyzer plate for bioenergetics and oxidative burst analysis.
Each stage of the procedure should be performed in sterile conditions and is encouraged to prevent the premature activation of the oxidative burst response in monocytes and neutrophils. An indicator of less than sterile conditions during the isolation is evident when neutrophils, which have little to no oxygen consumption under basal conditions, begin the extracellular flux assay with elevated OCR measurements that gradually increase or decline throughout the assay. We stress the importance of imaging cells using light microscopy at 200X&#160;or greater to ensure that no morphological signs of activation have occurred prior to the assay. For example, neutrophils normally display a rounded to irregular shape with pronounced cell boundaries as seen in Figure 1B. However, these cells will flatten against the surface of the plate when activated and lose their distinct cell morphology. We have previously reported the morphological changes of activated leukocytes and platelets using this protocol and additional measures must be taken to ensure sterile conditions if encountering activation8.
A simplified scheme of the protocol is seen in Figure 2 as a time table in which the primary steps of the cell isolation, XF plate preparation, and XF assay are detailed. Isolation consists of the density gradient separation of cell types and is followed by magnetic separation. Parallel to the cell isolation process, XF plate preparation is necessary to avoid delays in cell plating or beginning the XF assay. This is critical because significant delays can lead to cell activation and diminished bioenergetics parameters.
Inadequate cell concentrations after isolation are a common problem and optimization of each centrifugation process is necessary to avoid cell loss. Successful isolations have been performed on as little as 6 ml of blood but alterations can be made depending on circulating concentrations of the desired cell type. If the density gradient is improperly prepared, distinct cell phases might not be visible and loss of cells can occur (see JoVE instructional video for a visual demonstration). Insufficient platelet isolated from the PRP is rare but has occurred if washing buffer does not contain PGI2 or if the isolation takes place below room temperature. The risk of platelet activation is often prevented if platelets are the last cells to be isolated; however, if platelets remain in washing buffer for extended periods the bioenergetics will be affected. There have been instances of smaller platelet populations that did not pellet during the 1,500 x g centrifugation and the bioenergetics of these cells has not been extensively characterized. See Table 2 for a more complete troubleshooting guide.
The bioenergetic profiles of leukocytes and platelets can be determined using the XF analyzer, which measures real-time O2 consumption in cells noninvasively. Each cell type is plated on the XF24 plate with five replicates as shown in the Figure 3A. Table 1 indicates the expected basal and oxidative burst values by cell type during the assay and the average protein concentrations per well. Higher throughput technologies are available, such as the XF96, which allows for four donors to be assessed simultaneously as shown in Figure 3B. After the assay, the data is exported to a work-station computer for analysis using the appropriate XF software and Microsoft excel. The OCR values were normalized to total protein content in the corresponding wells and expressed as pmol/min/mg protein. The representative bioenergetic-oxidative burst profiles of each cell type were recently reported by our group8. Further analysis of bioenergetic parameters of the assay (basal, ATP-linked, proton leak, maximal, nonmitochondrial and oxidative burst) can be calculated for individual wells as previously shown and described below8.
The basal oxygen consumption rate (OCR) is established by the first 3 measurements as shown in Figure 4A. Oligomycin (0.5 &#181;g/ml), an inhibitor of mitochondrial ATP-synthase is injected into the XF medium to estimate the OCR coupled to ATP synthesis and represented as ATP-linked. The residual OCR minus the nonmitochondrial OCR can be attributed to proton leak. Then FCCP an uncoupler is added to determine the maximal OCR, followed by antimycin-A, an inhibitor of mitochondrial respiration, to determine nonmitochondrial sources of oxygen consumption. Reserve capacity is a measure of the amount of ATP that can be produced under energetic demand and can be calculated as the difference between the maximum rate of respiration and the basal. In order to determine the oxidative burst capacity, phorbol 12-myristate 13-acetate (PMA) a PKC agonist is injected to increase NADPH oxidase activity, and the increase in oxygen consumption rate following PMA stimulation can be measured using the XF analyzer. Figure 4B show how to calculate the different parameters of mitochondrial function and oxidative burst.
<img alt="Figure 1" fo:content-width="5in" fo:src="/files/ftp_upload/51301/51301fig1highres.jpg" src="/files/ftp_upload/51301/51301fig1.jpg" /> 
Figure 1. Isolation of Leukocytes and Platelets from Whole Blood. A) Freshly collected specimens are separated into their plasma and cellular components by centrifugation and purified by Ficoll density gradient, and Magnetic Activated Cell Sorting (MACS) by positive (monocyte and neutrophil) or negative selection (lymphocytes), while platelets are isolated by high-speed centrifugation of the platelet rich plasma. B) Images of the isolated cell populations once resuspended in XF DMEM and plated at indicated cell densities. <a href="https://www.jove.com/files/ftp_upload/51301/51301fig1highres.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" fo:content-width="5in" fo:src="/files/ftp_upload/51301/51301fig2highres.jpg" src="/files/ftp_upload/51301/51301fig2.jpg" /> 
Figure 2. Preparation of XF24 plates for Bioenergetic studies of leukocytes and platelets. Detailed timeline for the preparation of a XF24 assay plate by cell isolation and plating and cartridge hydration and injection port loading.
<img alt="Figure 3" fo:content-width="5in" fo:src="/files/ftp_upload/51301/51301fig3highres.jpg" src="/files/ftp_upload/51301/51301fig3.jpg" /> 
Figure 3. Layout of leukocytes and platelets on XF24 and XF96 analyzer plates. A) Leukocytes (125-250k cells/well) and platelets (25 x 106 cells/well) from a single donor are plated on the XF24 assay plate among background controls. 75 &#181;l of 10x stocks of oligomycin (0.5 &#181;g / ml), FCCP (0.6 &#181;M), antimycin-A (10 &#181;M), and PMA (100 ng/ml) diluted in XF media are loaded into the indicated injection ports. B) Leukocytes (75-150k cells/well) and platelets (10 x106 cells/well) from as many as four donors can be plated on the XF96 in a total volume of 180 &#181;l XF-DMEM. 20 &#181;l of 10x stocks of oligomycin (1.0 &#181;g/ml), FCCP (0.6 &#181;M), antimycin-A (10 &#181;M), and PMA (100 ng/ml) diluted in XF-DMEM are loaded into the indicated injection ports.
<img alt="Figure 4" fo:content-width="5in" fo:src="/files/ftp_upload/51301/51301fig4highres.jpg" src="/files/ftp_upload/51301/51301fig4.jpg" /> 
Figure 4. Analysis of Bioenergetic indices. A) Representative trace of oxygen consumption rate (OCR) by mitochondria and oxidative burst in monocytes. Basal OCR is established (first 3 rates indicated by numbers in circles). Then sequential additions of oligomycin (O; 0.5 &#181;g/ml), FCCP (F; 0.6 &#181;M) and antimycin-A (A; 10 &#181;M) are injected to determine mitochondrial and nonmitochondrial respiration of nonactivated cells. Finally, PMA (100 ng/ml) is added to measure oxidative burst.&#160;B) Modular analysis of mitochondrial function and oxidative burst are calculated by the differences in the rates as indicated.
<table border="0" cellpadding="0" cellspacing="0">
	<tbody>
		<tr height="66">
			<td height="66" style="height:67px;width:215px;"></td>
			<td style="width:215px;">Optimal Seeding Density</td>
			<td style="width:215px;">Avg. Basal OCR (pmol O2/min)</td>
			<td style="width:215px;">Avg. Oxidative Burst OCR (pmol O2/min)</td>
			<td style="width:215px;">Avg. protein (&#181;g)/well</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Monocytes</td>
			<td>250k cells / well</td>
			<td>83.9 ( &#177; 13.0)</td>
			<td>300.3 ( &#177; 58.8)</td>
			<td>19.0 ( &#177; 2.4)</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Neutrophils</td>
			<td>250k cells / well</td>
			<td>6.1 ( &#177; 2.2)</td>
			<td>1411.8 ( &#177; 233.3)</td>
			<td>20.6 ( &#177; 2.7)</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Lymphocytes</td>
			<td>250k cells / well</td>
			<td>52.9 ( &#177; 7.7)</td>
			<td>15 ( &#177; 4.1)</td>
			<td>13.2 ( &#177; 2.1)</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Platelets</td>
			<td>25 x 106 cells / well</td>
			<td>199.4 ( &#177; 20.3)</td>
			<td>24 ( &#177; 2.7)</td>
			<td>47.5 ( &#177; 3.1)</td>
		</tr>
	</tbody>
</table>
Table 1.&#160;Normal parameters for the XF24 assay: The average basal (Rate 3) and oxidative burst (Rate 7) OCR not corrected to nonmitochondrial OCR or protein are shown by cell type plated at the indicated cell densities. The average protein content per well is shown as performed by a DC Lowry assay. These data represent the mean values of 6-8 healthy donors with parenthesis containing &#177; SEM.
<table border="0" cellpadding="0" cellspacing="0">
	<colgroup>
		<col span="4" />
	</colgroup>
	<tbody>
		<tr height="66">
			<td>Step</td>
			<td>Problem</td>
			<td>Possible reason</td>
			<td>Solution</td>
		</tr>
		<tr height="66">
			<td height="66" style="height:67px;width:199px;">1.2</td>
			<td style="width:199px;">clear plasma</td>
			<td style="width:199px;">platelets pelleted during centrifugation</td>
			<td style="width:199px;">decrease centrifugation time to 10 min or slow to 400 x g</td>
		</tr>
		<tr height="66">
			<td height="66" style="height:67px;width:199px;"></td>
			<td style="width:199px;">milky plasma</td>
			<td style="width:199px;">excess lipids</td>
			<td style="width:199px;">avoid postprandial collection</td>
		</tr>
		<tr height="66">
			<td height="66" style="height:67px;width:199px;">1.6</td>
			<td style="width:199px;">incomplete cell bands formed&#160;</td>
			<td style="width:199px;">improper gradient preparation, cold reagent</td>
			<td style="width:199px;">avoid disrupting gradient during pipetting, use room temperature reagent</td>
		</tr>
		<tr height="66">
			<td height="66" style="height:67px;width:199px;"></td>
			<td style="width:199px;">clumps in cell bands</td>
			<td style="width:199px;">clotting of blood may have occurred</td>
			<td style="width:199px;">Collect blood using anticoagulants such as ACD or EDTA&#160;</td>
		</tr>
		<tr height="66">
			<td height="66" style="height:67px;width:199px;">1.10</td>
			<td style="width:199px;">no cell pellet</td>
			<td style="width:199px;">see step 1.6</td>
			<td style="width:199px;">If supernatant hazy see below</td>
		</tr>
		<tr height="66">
			<td height="66" style="height:67px;width:199px;"></td>
			<td style="width:199px;">hazy supernatant</td>
			<td style="width:199px;">Heavy Ficoll gradient contamination, platelet contamination</td>
			<td style="width:199px;">Increase centrifugation speed to 900 x g, dilute with more RPMI</td>
		</tr>
		<tr height="66">
			<td height="66" style="height:67px;width:199px;">1.16, 1.17</td>
			<td style="width:199px;">low yield of leukocytes</td>
			<td style="width:199px;">heavy RBC contamination, not enough whole blood, clotting</td>
			<td style="width:199px;">Double antibody and RPMI-BSA volumes, collect more blood, add anticoagulant</td>
		</tr>
		<tr height="66">
			<td height="66" style="height:67px;width:199px;">1.19</td>
			<td style="width:199px;">platelet aggregation</td>
			<td style="width:199px;">PGI2 omitted, exposure to cold media, prolonged storage in plasma</td>
			<td style="width:199px;">add PGI2 to platelet wash buffer, use room temperature reagents</td>
		</tr>
		<tr height="66">
			<td height="66" style="height:67px;width:199px;">1.20</td>
			<td style="width:199px;">low platelet count</td>
			<td style="width:199px;">loss during primary centrifugation, platelet aggregation</td>
			<td style="width:199px;">See steps 1.2 and 1.19</td>
		</tr>
		<tr height="66">
			<td height="66" style="height:67px;width:199px;">2.3</td>
			<td style="width:199px;">RBC contamination</td>
			<td style="width:199px;"></td>
			<td style="width:199px;">Repeat MACS separation</td>
		</tr>
	</tbody>
</table>
Table 2.&#160;Leukocyte and platelet isolation troubleshooting.&#160;The table lists common problems encountered during leukocyte and platelet cell isolation from whole blood and solutions that may guide users through the troubleshooting process.

Watch this Scientific Journal Video about Bioenergetics and the Oxidative Burst: Protocols for the Isolation and Evaluation of Human Leukocytes and Platelets at JoVE.com

Bioenergetics and the Oxidative Burst: Protocols for the Isolation and Evaluation of Human Leukocytes and Platelets

Blood leukocytes and platelets can be used as a marker of overall bioenergetic health of an individual and so have the potential to monitor pathological processes and the impact of treatments. Here&#160;we describe a method to isolate and measure mitochondrial function and the oxidative burst in these cells.

Mitochondrial dysfunction is known to play a significant role in a number of pathological conditions such as atherosclerosis, diabetes, septic shock, and ...

bioenergetics-oxidative-burst-protocols-for-isolation-evaluation

Research

JoVE Journal

Immunology and Infection

37.0K 次观看.  University of Alabama at Birmingham. 血液白细胞和血小板可以作为一个单独的整体生物能量健康的一个标志，所以具有监视病理过程和治疗的影响的可能性。这里我们描述的方法来分离并测量线粒体功能和在这些细胞中的氧化爆发。 

视频: Bioenergetics and the Oxidative Burst: Protocols for the Isolation and Evaluation of Human Leukocytes and Platelets

Isolation of Brain-infiltrating Leukocytes

We describe a method for preparing brain infiltrating leukocytes (BILs) from mice. We demonstrate how to infect mice with Theiler's murine encephalomyelitis virus (TMEV) via a rapid intracranial injection technique and how to purify a leukocyte-enriched population of infiltrating cells from whole brain. Briefly, mice are anesthetized with isoflurane in a closed chamber and are free-hand injected with a Hamilton syringe into the frontal cortex. Mice are then killed at various times after infection by isoflurane overdose and whole brains are extracted and homogenized in RPMI with a Tenbroeck tissue grinder. Brain homogenates are centrifuged through a continuous 30% Percoll gradient to remove the myelin and other cell debris. The cell suspension is then strained at 40 &mu;m, washed and centrifuged on a discontinuous Ficoll-Paque Plus gradient to select and purify the leukocytes. The leukocytes are then washed and resuspended in appropriate buffers for immunophenotyping by flow cytometry. Flow cytometry reveals a population of innate immune cells at the early stages of infection in C57BL/6 mice. At 24 hours post infection, multiple subsets of immune cells are present in the BILs, with an enriched population of Gr1+, CD11b+ and F4/80+cells. Therefore, this method is useful in characterizing the immune response to acute infection in the brain.

A rapid method to obtain infiltrating leukocytes from the murine brain is described. This method utilizes a continuous Percoll gradient and discontinuous Ficoll gradient to select and purify the leukocyte-enriched layer. Isolated leukocytes may then be characterized by flow cytometric measurements.

We describe a method for preparing brain infiltrating leukocytes (BILs) from mice. We demonstrate how to infect mice with Theiler's murine ...

Isolation and Analysis of Brain-sequestered Leukocytes from Plasmodium berghei ANKA-infected Mice

We describe a method for isolation and characterization of adherent inflammatory cells from brain blood vessels of P. berghei ANKA-infected mice. Infection of susceptible mouse-strains with this parasite strain results in the induction of experimental cerebral malaria, a neurologic syndrome that recapitulates certain important aspects of Plasmodium falciparum-mediated severe malaria in humans 1,2 . Mature forms of blood-stage malaria express parasitic proteins on the surface of the infected erythrocyte, which allows them to bind to vascular endothelial cells. This process induces obstructions in blood flow, resulting in hypoxia and haemorrhages 3 and also stimulates the recruitment of inflammatory leukocytes to the site of parasite sequestration.
Unlike other infections, i.e neutrotopic viruses4-6, both malaria-parasitized red blood cells (pRBC) as well as associated inflammatory leukocytes remain sequestered within blood vessels rather than infiltrating the brain parenchyma. Thus to avoid contamination of sequestered leukocytes with non-inflammatory circulating cells, extensive intracardial perfusion of infected-mice prior to organ extraction and tissue processing is required in this procedure to remove the blood compartment. After perfusion, brains are harvested and dissected in small pieces. The tissue structure is further disrupted by enzymatic treatment with Collagenase D and DNAse I. The resulting brain homogenate is then centrifuged on a Percoll gradient that allows separation of brain-sequestered leukocytes (BSL) from myelin and other tissue debris. Isolated cells are then washed, counted using a hemocytometer and stained with fluorescent antibodies for subsequent analysis by flow cytometry.
This procedure allows comprehensive phenotypic characterization of inflammatory leukocytes migrating to the brain in response to various stimuli, including stroke as well as viral or parasitic infections. The method also provides a useful tool for assessment of novel anti-inflammatory treatments in pre-clinical animal models.

Isolation and Analysis of Brain-sequestered Leukocytes from Plasmodium berghei ANKA-infected Mice

A method for isolation of adherent inflammatory leukocytes from brain blood vessels of Plasmodium berghei ANKA-infected mice is described. The method allows quantification as well as phenotypic characterization of isolated leukocytes after staining with fluorescent antibodies and subsequent analysis by flow cytometry.

We describe a method for isolation and  characterization of adherent inflammatory cells from brain blood vessels of P. berghei ANKA-infected mice. ...

Analyzing the Effects of Stromal Cells on the Recruitment of Leukocytes from Flow

Stromal cells regulate the recruitment of circulating leukocytes during inflammation through cross-talk with neighboring endothelial cells. Here we describe two in vitro &#8220;vascular&#8221; models for studying the recruitment of circulating neutrophils from flow by inflamed endothelial cells. A major advantage of these models is the ability to analyze each step in the leukocyte adhesion cascade in order, as would occur in vivo. We also describe how both models can be adapted to study the role of stromal cells, in this case mesenchymal stem cells (MSC), in regulating leukocyte recruitment.
Primary endothelial cells were cultured alone or together with human MSC in direct contact on Ibidi microslides or on opposite sides of a Transwell filter for 24 hr. Cultures were stimulated with tumor necrosis factor alpha (TNF&#945;) for 4 hr and incorporated into a flow-based adhesion assay. A bolus of neutrophils was perfused over the endothelium for 4 min. The capture of flowing neutrophils and their interactions with the endothelium was visualized by phase-contrast microscopy.
In both models, cytokine-stimulation increased endothelial recruitment of flowing neutrophils in a dose-dependent manner. Analysis of the behavior of recruited neutrophils showed a dose-dependent decrease in rolling and a dose-dependent increase in transmigration through the endothelium. In co-culture, MSC suppressed neutrophil adhesion to TNF&#945;-stimulated endothelium.
Our flow based-adhesion models mimic the initial phases of leukocyte recruitment from the circulation. In addition to leukocytes, they can be used to examine the recruitment of other cell types, such as therapeutically administered MSC or circulating tumor cells. Our multi-layered co-culture models have shown that MSC communicate with endothelium to modify their response to pro-inflammatory cytokines, altering the recruitment of neutrophils. Further research using such models is required to fully understand how stromal cells from different tissues and conditions (inflammatory disorders or cancer) influence the recruitment of leukocytes during inflammation.

The ability of inflamed endothelium to recruit leukocytes from flow is regulated by mesenchymal stromal cells. We describe two in vitro models incorporating primary human cells that can be used to assess neutrophil recruitment from flow and examine the role that mesenchymal stromal cells play in regulating this process.

Stromal cells regulate the recruitment of circulating leukocytes during inflammation through cross-talk with neighboring endothelial cells. Here we ...

Isolation of Leukocytes from the Human Maternal-fetal Interface

Pregnancy is characterized by the infiltration of leukocytes in the reproductive tissues and at the maternal-fetal interface (decidua basalis and decidua parietalis). This interface is the anatomical site of contact between maternal and fetal tissues; therefore, it is an immunological site of action during pregnancy. Infiltrating leukocytes at the maternal-fetal interface play a central role in implantation, pregnancy maintenance, and timing of delivery. Therefore, phenotypic and functional characterizations of these leukocytes will provide insight into the mechanisms that lead to&#160;pregnancy disorders. Several protocols have been described in order to isolate infiltrating leukocytes from the decidua basalis and decidua parietalis; however, the lack of consistency in the reagents, enzymes, and times of incubation makes it difficult to compare these results. Described herein is&#160;a novel approach that combines the use of gentle mechanical and enzymatic dissociation techniques to preserve the viability and integrity of extracellular and intracellular markers in leukocytes isolated from the human tissues at the maternal-fetal interface. Aside from immunophenotyping, cell culture, and cell sorting, the future applications of this protocol are numerous and varied. Following this protocol, the isolated leukocytes can be used to determine DNA methylation, expression of target genes, in vitro leukocyte functionality (i.e., phagocytosis, cytotoxicity, T-cell proliferation, and plasticity, etc.), and the production of reactive oxygen species at the maternal-fetal interface. Additionally, using the described protocol, this laboratory has been able to describe new and rare leukocytes at the maternal-fetal interface.

Described herein is a protocol to isolate and further study the infiltrating leukocytes of the decidua basalis and decidua parietalis - the human maternal-fetal interface. This protocol maintains the integrity of cell surface markers and yields enough viable cells for downstream applications as proven by flow cytometry analysis.

Pregnancy is characterized by the infiltration of leukocytes in the reproductive tissues and at the maternal-fetal interface (decidua basalis and decidua ...

Isolation of Leukocytes from the Murine Tissues at the Maternal-Fetal Interface

Immune tolerance in pregnancy requires that the immune system of the mother undergoes distinctive changes in order to accept and nurture the developing fetus. This tolerance is initiated during coitus, established during fecundation and implantation, and maintained throughout pregnancy. Active cellular and molecular mediators of maternal-fetal tolerance are enriched at the site of contact between fetal and maternal tissues, known as the maternal-fetal interface, which includes the placenta and the uterine and decidual tissues. This interface is comprised of stromal cells and infiltrating leukocytes, and their abundance and phenotypic characteristics change over the course of pregnancy. Infiltrating leukocytes at the maternal-fetal interface include neutrophils, macrophages, dendritic cells, mast cells, T cells, B cells, NK cells, and NKT cells that together create the local micro-environment that sustains pregnancy. An imbalance among these cells or any inappropriate alteration in their phenotypes is considered a mechanism of disease in pregnancy. Therefore, the study of leukocytes that infiltrate the maternal-fetal interface is essential in order to elucidate the immune mechanisms that lead to pregnancy-related complications. Described herein is a protocol that uses a combination of gentle mechanical dissociation followed by a robust enzymatic disaggregation with a proteolytic and collagenolytic enzymatic cocktail to isolate the infiltrating leukocytes from the murine tissues at the maternal-fetal interface. This protocol allows for the isolation of high numbers of viable leukocytes (&#62;70%) with sufficiently conserved antigenic and functional properties. Isolated leukocytes can then be analyzed by several techniques, including immunophenotyping, cell sorting, imaging, immunoblotting, mRNA expression, cell culture, and in vitro functional assays such as mixed leukocyte reactions, proliferation, or cytotoxicity assays.

Described herein is a protocol to isolate and analyze the infiltrating leukocytes of tissues at the maternal-fetal interface (uterus, decidua, and placenta) of mice. This protocol maintains the integrity of most cell surface markers and yields enough viable cells for downstream applications including flow cytometry analysis.

Immune tolerance in pregnancy requires that the immune system of the mother undergoes distinctive changes in order to accept and nurture the developing ...

Isolation of Infiltrating Leukocytes from Mouse Skin Using Enzymatic Digest and Gradient Separation

Dissociating murine skin into a single cell suspension is essential for downstream cellular analysis such as the characterization of infiltrating immune cells in rodent models of skin inflammation. Here, we describe a protocol for the digestion of mouse skin in a nutrient-rich solution with collagenase D, followed by separation of hematopoietic cells using a discontinuous density gradient. Cells thus obtained can be used for in vitro studies, in vivo transfer, and other downstream cellular and molecular analyses including flow cytometry. This protocol is an effective and economical alternative to expensive mechanical dissociators, specialized separation columns, and harsher trypsin- and dispase-based digestion methods, which may compromise cellular viability or density of surface proteins relevant for phenotypic characterization or cellular function. As shown here in our representative data, this protocol produced highly viable cells, contained specific immune cell subsets, and had no effect on integrity of common surface marker proteins used in flow cytometric analysis.

This protocol describes enzymatic digestion of mouse skin in nutrient-rich medium followed by gradient separation to isolate leukocytes. Cells thus derived can be used for diverse downstream applications. This is an effective, economical, and improved alternative to tissue dissociation machines and harsher trypsin and dispase-based tissue digestion protocols.

Dissociating murine skin into a single cell suspension is essential for downstream cellular analysis such as the characterization of infiltrating immune ...

Measuring Granulocyte and Monocyte Phagocytosis and Oxidative Burst Activity in Human Blood

The granulocyte and monocyte phagocytosis and oxidative burst (OB) activity assay can be used to study the innate immune system. This manuscript provides the necessary methodology to add this assay to an exercise immunology arsenal. The first step in this assay is to prepare two aliquots ("H" and "F") of whole blood (heparin). Then, dihydroethidium is added to the H aliquot, and both aliquots are incubated in a warm water bath followed by a cold water bath. Next, Staphylococcus aureus (S. aureus) is added to the H aliquot and fluorescein isothiocyanate-labeled S. aureus is added to the F aliquot (bacteria:phagocyte = 8:1), and both aliquots are incubated in a warm water bath followed by a cold water bath. Then, trypan blue is added to each aliquot to quench extracellular fluorescence, and the cells are washed with phosphate-buffered saline. Next, the red blood cells are lysed, and the white blood cells are fixed. Finally, a flow cytometer and appropriate analysis software are used to measure granulocyte and monocyte phagocytosis and OB activity. This assay has been used for over 20 years. After heavy and prolonged exertion, athletes experience a significant but transient increase in phagocytosis and an extended decrease in OB activity. The post-exercise increase in phagocytosis is correlated with inflammation. In contrast to normal weight individuals, granulocyte and monocyte phagocytosis is chronically elevated in overweight and obese participants, and is modestly correlated with C-reactive protein. In summary, this flow cytometry-based assay measures the phagocytosis and OB activity of phagocytes and can be used as an additional measure of exercise- and obesity-induced inflammation.

The purpose of this manuscript is to present a method for measuring monocyte and granulocyte phagocytosis and oxidative burst activity in human blood samples.

The granulocyte and monocyte phagocytosis and oxidative burst (OB) activity assay can be used to study the innate immune system. This manuscript provides ...

Two-photon Intravital Imaging of Leukocytes During the Immune Response in Lipopolysaccharide-treated Mouse Liver

Sepsis is a type of severe infection that can cause organ failure and tissue damage. Although the mortality and morbidity rates associated with sepsis are extremely high, no direct treatment or organ-related mechanism has been examined in detail in real time. The liver is the key organ that manages toxins and infections in the human body. Herein, we aimed to perform intravital imaging of mouse liver after induction of endotoxemia in order to track the motility of immune cells, such as neutrophils and liver capsular macrophages (LCMs). Accordingly, we designed a novel surgical method for exposure of the liver with minimally invasive surgery. Mice were intraperitoneally injected with lipopolysaccharide (LPS), a common endotoxin. Using our novel surgical approach for exposure and intravital imaging of the mouse liver, we found that neutrophil recruitment in LPS-treated LysM-green fluorescent protein (GFP) mouse liver was increased compared with that in phosphate-buffered saline-treated liver. After LPS treatment, the number of neutrophils increased significantly with time. Additionally, using CX3Cr1-GFP mice, we successfully visualized liver resident macrophages called LCMs. Therefore, to investigate the efficacy of new reagents to control immune mobility in vivo, determining the motility and morphology of neutrophils and LCMs in the liver may allow us to identify therapeutic effect in organ failure and tissue damage caused by leukocytes activation in sepsis.

We established a novel surgical protocol for two-photon imaging of live mice liver with minimal invasion. With this technique, we identified the detailed structure of the liver during lipopolysaccharide-induced endotoxemia. We anticipate that this method may be utilized to determine the effectiveness of various reagents treatment to hepatic leukocyte migration.

Sepsis is a type of severe infection that can cause organ failure and tissue damage. Although the mortality and morbidity rates associated with sepsis are ...

Evaluation of Host-Pathogen Responses and Vaccine Efficacy in Mice

Vaccines are a 20th century medical marvel. They have dramatically reduced the morbidity and mortality caused by infectious diseases and contributed to a striking increase in life expectancy around the globe. Nonetheless, determining vaccine efficacy remains a challenge. Emerging evidence suggests that the current acellular vaccine (aPV) for Bordetella pertussis (B. pertussis) induces suboptimal immunity. Therefore, a major challenge is designing a next-generation vaccine that induces protective immunity without the adverse side effects of a whole-cell vaccine (wPV). Here we describe a protocol that we used to test the efficacy of a promising, novel adjuvant that skews immune responses to a protective Th1/Th17 phenotype and promotes a better clearance of a B. pertussis challenge from the murine respiratory tract. This article describes the protocol for mouse immunization, bacterial inoculation, tissue harvesting, and analysis of immune responses. Using this method, within our model, we have successfully elucidated crucial mechanisms elicited by a promising, next-generation acellular pertussis vaccine. This method can be applied to any infectious disease model in order to determine vaccine efficacy.

Here we present an elegant protocol for in vivo evaluation of vaccine effectiveness and host immune responses. This protocol can be adapted for vaccine models that study viral, bacterial, or parasitic pathogens.

Vaccines are a 20th century medical marvel. They have dramatically reduced the morbidity and mortality caused by infectious diseases and contributed to a ...

Pattern-Triggered Oxidative Burst and Seedling Growth Inhibition Assays in Arabidopsis thaliana

Plants have evolved a robust immune system to perceive pathogens and protect against disease. This paper describes two assays that can be used to measure the strength of immune activation in Arabidopsis thaliana following treatment with elicitor molecules. Presented first is a method for capturing the rapidly-induced and dynamic oxidative burst, which can be monitored using a luminol-based assay. Presented second is a method describing how to measure immune-induced inhibition of seedling growth. These protocols are fast and reliable, do not require specialized training or equipment, and are widely used to understand the genetic basis of plant immunity.

Pattern-Triggered Oxidative Burst and Seedling Growth Inhibition Assays in Arabidopsis thaliana

This paper describes two methods for quantifying defense responses in Arabidopsis thaliana following exposure to immune elicitors: the transient oxidative burst, and the inhibition of seedling growth.

Plants have evolved a robust immune system to perceive pathogens and protect against disease. This paper describes two assays that can be used to measure ...