This work was funded by the Health Research Board EIA-2024-002 and the Royal City of Dublin Hospital Trust. We would like to thank Dr. Lorraine Thong and Dr. Kevin Brown for their assistance in collecting samples from healthy donors for this manuscript.

Blood samples were collected with informed consent from healthy participants. The study received approval from the Research Ethics Committee of both St. James&#39;s Hospital and Tallaght University Hospital.
1. Preparation of density gradient medium, isotonic working solutions fractions and cell separation buffer
<ol>
	<li>Preparation of isotonic working solutions from density gradient medium
	<ol>
		<li>Preparation of Isotonic 100% working solution (~1.123 g/mL)
		<ol>
			<li>To prepare the isotonic 100% working solution, combine 27 mL of density gradient medium with 3 mL of 10x PBS. This results in an isotonic solution suitable for further dilutions.</li>
		</ol>
		</li>
		<li>Preparation of isotonic 81% working solution (~1.0996 g/mL)
		<ol>
			<li>Prepare the isotonic 81% working solution by mixing 8.1 mL of the isotonic 100% working solution (prepared in step 1.1.1) with 1.9 mL of 1x PBS. Mix thoroughly to ensure homogeneity.</li>
		</ol>
		</li>
		<li>Preparation of isotonic 70% working solution (~1.0861 g/mL)
		<ol>
			<li>To prepare the isotonic 70% working solution, combine 7 mL of the isotonic 100% working solution with 3 mL of 1x PBS. Ensure that the solution is well mixed.</li>
		</ol>
		</li>
		<li>Preparation of isotonic 55% working solution (1.0676 g/mL)
		<ol>
			<li>Make the isotonic 55% working solution by mixing 5.5 mL of the isotonic 100% working solution with 4.5 mL of 1x PBS. Mix thoroughly.</li>
		</ol>
		</li>
	</ol>
	</li>
	<li>Layering of gradient fractions
	<ol>
		<li>Gradient fraction layering
		<ol>
			<li>Using a 15 mL conical tube, carefully layer 3 mL of the isotonic 81% working solution at the bottom. Then, slowly and gently layer 3 mL of the isotonic 70% working solution on top, avoiding mixing the layers. This gradient will be used for cell separation.</li>
		</ol>
		</li>
	</ol>
	</li>
	<li>Preparation of cell separation buffer
	<ol>
		<li>Preparation of 500 mL of cell separation buffer
		<ol>
			<li>To prepare the cell separation buffer, combine 2% fetal bovine serum (FBS) and 1 mM ethylenediaminetetraacetic acid(EDTA) with 1x PBS to a total volume of 500 mL. Use this buffer to wash and resuspend cells during the isolation process. 
			NOTE: Ensure that the layers are well-separated and undisturbed. In this protocol, the isotonic working solutions are referred to as &#34;100%&#34;, &#34;81%&#34;, &#34;70%&#34;, and &#34;55%&#34; based on the method of preparation, consistent with previous studies5. However, it is important to clarify that these labels do not represent the actual final concentrations of the working solutions. For example, the &#34;100%&#34; density gradient medium is prepared by mixing 27 mL of pure density gradient medium with 3 mL of 10x PBS, resulting in a final concentration of 90% Isotonic working solution. The subsequent dilutions (e.g., &#34;81%&#34;, &#34;70%&#34;, and &#34;55%&#34;) similarly reflect preparation ratios rather than true percentage concentrations. This nomenclature was retained to maintain consistency with the terminology used in earlier literature on the subject.</li>
		</ol>
		</li>
	</ol>
	</li>
</ol>
2. Isolation of neutrophils from whole blood using negative selection
<ol>
	<li>Preparation of magnetic beads
	<ol>
		<li>Vortex the magnetic beads thoroughly for 30 s to ensure they are fully resuspended before use.</li>
	</ol>
	</li>
	<li>Blood preparation
	<ol>
		<li>For each donor, aliquot 4 mL of whole blood into three separate 14 mL round-bottomed tubes.</li>
	</ol>
	</li>
	<li>Addition of neutrophil isolation cocktail and magnetic beads
	<ol>
		<li>Add 50 &#181;L of neutrophil isolation cocktail and 50 &#181;L of magnetic beads per mL of blood to each tube. For 4 mL of blood, add 200 &#181;L of each reagent.</li>
		<li>Resuspend the mixture well by gently pipetting and incubate at room temperature (RT) for 5 min to allow the reagents to bind to unwanted cells.</li>
	</ol>
	</li>
	<li>Washing and magnetic separation - first round
	<ol>
		<li>Top up each tube to 12 mL using cell separation buffer and mix thoroughly.</li>
		<li>Place the tubes without lids on a magnet and let them incubate at RT for 10 min to allow the magnetic beads bound to unwanted cells to be drawn to the tube wall.</li>
	</ol>
	</li>
	<li>Collection of unbound cells
	<ol>
		<li>Carefully transfer the clear cell suspension containing neutrophils from each tube into a new, clean tube using a transfer pipette. Remove the original tube from the magnet.</li>
	</ol>
	</li>
	<li>Magnetic bead reapplication and incubation - second round
	<ol>
		<li>Vortex the magnetic beads again for 30 s. Add the same volume of magnetic beads to the newly transferred cell suspension as in step 2.3. Resuspend thoroughly and incubate at RT for another 5 min.</li>
	</ol>
	</li>
	<li>Final magnetic separation and collection
	<ol>
		<li>Place the tubes back onto the magnet without lids and incubate at RT for another 10 min.</li>
		<li>Carefully transfer the clear cell suspension to a new tube. This final suspension represents the isolated total neutrophil population.</li>
	</ol>
	</li>
</ol>
3. Separation of low-density neutrophils (LDNs) and normal-density neutrophils (NDNs) from the total neutrophil population
<ol>
	<li>Pooling and preparation of cell suspensions
	<ol>
		<li>For each donor, pool the isolated neutrophil suspensions into 50 mL tubes. Top up each tube to a total volume of 50 mL using the cell separation buffer.</li>
	</ol>
	</li>
	<li>Centrifugation
	<ol>
		<li>Centrifuge the tubes at 400&#160;x g for 5 min at RT with the brake on.</li>
	</ol>
	</li>
	<li>Resuspension and cell counting
	<ol>
		<li>Discard the supernatant and resuspend the neutrophil pellet in 1 mL of cell separation buffer. Perform a cell count to determine the total number of neutrophils.</li>
	</ol>
	</li>
	<li>Density gradient medium preparation
	<ol>
		<li>Centrifuge the tubes again at 400 x g for 5 min at RT with the brake on. Discard the supernatant and resuspend the neutrophil pellet in 3 mL of the 55% density gradient medium. For optimal resolution, use 3 mL of 55% density gradient medium per 5-6&#160;&#215; 106 total neutrophils.</li>
		<li>If necessary, divide the resuspended cells across multiple pre-made density gradient tubes, ensuring that 3 mL of the cell suspension is layered into each tube.</li>
	</ol>
	</li>
	<li>Layering onto density gradient tubes
	<ol>
		<li>Slowly layer the 3 mL cell suspension containing the 55% density gradient medium onto the pre-made density gradient tubes (prepared as described in section 1). Ensure careful layering to avoid disturbing the gradient.</li>
	</ol>
	</li>
	<li>Density gradient centrifugation
	<ol>
		<li>Centrifuge the tubes at 720 x g for 30 min without using the brake. After centrifugation, handle the tubes carefully to avoid disturbing the layers.</li>
	</ol>
	</li>
	<li>Isolation of neutrophil fractions
	<ol>
		<li>Following centrifugation, observe the neutrophils separate into two distinct layers: 
		Low-density neutrophils (LDNs) will be located at the 55%/70% interface, forming an upper band at approximately the 3 mL mark, and normal-density neutrophils (NDNs) will be at the 70%/81% interface, appearing as a lower band around the 6 mL mark.</li>
		<li>Using a transfer pipette, carefully isolate each layer and transfer them to separate 15 mL tubes.</li>
	</ol>
	</li>
	<li>Washing of isolated fractions
	<ol>
		<li>To wash off any residual density gradient medium, add 1x PBS to each 15 mL tube up to the 15 mL mark.</li>
		<li>Centrifuge at 400&#160;&#215; g for 5 min at RT with the brake on. If the cells do not form a firm pellet and instead remain suspended, repeat this wash step, indicating the presence of remaining density gradient medium.</li>
	</ol>
	</li>
	<li>Cell count and downstream applications
	<ol>
		<li>Count the cells in each fraction and proceed with downstream applications such as metabolic experiments, flow cytometry staining, RNA extraction, or protein lysis as needed. 
		NOTE: After plating cells out, spinning down the plate at 210&#160;&#215;&#160;g for 1 min (brake off) is recommended.</li>
	</ol>
	</li>
</ol>
4. Phenotyping of isolated LDN and NDN
<ol>
	<li>Isolate ~0.5-1&#160;&#215; 106 LDNs and NDNs. Make a 2x concentrated antibody mastermix using CD14, CD86, CD15, CD16, CD10, Fc block, and viability stain.</li>
	<li>Stain the isolated LDN and NDN populations with an equivalent volume of the antibody mastermix so that the final dilution of antibodies staining the cells is 1:100 (CD14, CD86, CD15, CD16, CD10, Fc block) and 1:50 (viability stain), respectively.</li>
	<li>Incubate the cells for 10 min in the dark at RT. 
	NOTE: Ensure the cells are thoroughly mixed with the antibody mastermix and Fc block.</li>
	<li>Wash the cells once with PBS, then centrifuge at 400&#160;&#215; g for 5 min. Discard the supernatant.</li>
	<li>Fix the cells in 1% paraformaldehyde (PFA) for 15 min at RT in the dark.</li>
	<li>Wash the cells again with PBS, centrifuge at 400&#160;&#215; g for 5 min, and discard the supernatant.</li>
	<li>Resuspend the cells in 200 &#181;L of PBS or as required to be used and acquire the cells on a flow cytometer as soon as possible. 
	NOTE: The stained and fixed cells can be stored short-term at 4 &#9702;C in the dark to prevent photobleaching the fluorophores. However, ideally, the phenotyping procedure should be carried out promptly after staining and fixation to ensure optimal cell viability and accurate results.</li>
</ol>

<ol>
	<li>Tracchi, I., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Increased+neutrophil+lifespan+in+patients+with+congestive+heart+failure.">Increased neutrophil lifespan in patients with congestive heart failure.</a> Eur J Heart Fail. 11 (4), 378-385 (2009).</li><li>Ballesteros, I., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Co-option+of+neutrophil+fates+by+tissue+environments.">Co-option of neutrophil fates by tissue environments.</a> Cell. 183 (5), 1282-1297.e18 (2020).</li><li>Mckenna, 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=Neutrophils:+Need+for+standardized+nomenclature.">Neutrophils: Need for standardized nomenclature.</a> Front Immunol. 12, 602963 (2021).</li><li>Hacbarth, E., Kajdacsy-Balla, A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Low+density+neutrophils+in+patients+with+systemic+lupus+erythematosus,+rheumatoid+arthritis,+and+acute+rheumatic+fever.">Low density neutrophils in patients with systemic lupus erythematosus, rheumatoid arthritis, and acute rheumatic fever.</a> Arthritis Rheumatol. 29 (11), 1334-1342 (1986).</li><li>Hardisty, G. 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=High+purity+isolation+of+low+density+neutrophils+casts+doubt+on+their+exceptionality+in+health+and+disease.">High purity isolation of low density neutrophils casts doubt on their exceptionality in health and disease.</a> Front Immunol. 12, 625922 (2021).</li><li>Scapini, P., Marini, O., Tecchio, C., Cassatella, M. A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Human+neutrophils+in+the+saga+of+cellular+heterogeneity:+Insights+and+open+questions.">Human neutrophils in the saga of cellular heterogeneity: Insights and open questions.</a> Immunol Rev. 273 (1), 48-60 (2016).</li><li>Ssemaganda, 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=Characterization+of+neutrophil+subsets+in+healthy+human+pregnancies.">Characterization of neutrophil subsets in healthy human pregnancies.</a> PLoS One. 9 (2), e85696 (2014).</li><li>Tay, S. H., Celhar, T., Fairhurst, A. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Low-density+neutrophils+in+systemic+lupus+erythematosus.">Low-density neutrophils in systemic lupus erythematosus.</a> Arthritis Rheumatol. 72 (10), 1587-1595 (2020).</li><li>Hassani, 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=On+the+origin+of+low-density+neutrophils.">On the origin of low-density neutrophils.</a> J Leukoc Biol. 107 (5), 809-818 (2020).</li><li>Cowland, J. B., Borregaard, N. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Isolation+of+neutrophil+precursors+from+bone+marrow+for+biochemical+and+transcriptional+analysis.">Isolation of neutrophil precursors from bone marrow for biochemical and transcriptional analysis.</a> J Immunol Methods. 232 (1-2), 191-200 (1999).</li><li>Blanco-Camarillo, C., Aleman, O. R., Rosales, C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Low-density+neutrophils+in+healthy+individuals+display+a+mature+primed+phenotype.">Low-density neutrophils in healthy individuals display a mature primed phenotype.</a> Front Immunol. 12, 672520 (2021).</li><li>Park, J., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Low-density+granulocytes+display+immature+cells+with+enhanced+NET+formation+in+people+living+with+HIV.">Low-density granulocytes display immature cells with enhanced NET formation in people living with HIV.</a> Sci Rep. 13 (1), 13282 (2023).</li><li>Denny, M. F., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+distinct+subset+of+proinflammatory+neutrophils+isolated+from+patients+with+systemic+lupus+erythematosus+induces+vascular+damage+and+synthesizes+type+I+IFNs.">A distinct subset of proinflammatory neutrophils isolated from patients with systemic lupus erythematosus induces vascular damage and synthesizes type I IFNs.</a> J Immunol. 184 (6), 3284-3297 (2010).</li><li>Ui Mhaonaigh, 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=Low+density+granulocytes+in+anca+vasculitis+are+heterogenous+and+hypo-responsive+to+anti-myeloperoxidase+antibodies.">Low density granulocytes in anca vasculitis are heterogenous and hypo-responsive to anti-myeloperoxidase antibodies.</a> Front Immunol. 10, 2603 (2019).</li><li>Mosca, T., Forte, W. C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Comparative+efficiency+and+impact+on+the+activity+of+blood+neutrophils+isolated+by+Percoll,+Ficoll+and+spontaneous+sedimentation+methods.">Comparative efficiency and impact on the activity of blood neutrophils isolated by Percoll, Ficoll and spontaneous sedimentation methods.</a> Immunol Invest. 45 (1), 29-37 (2016).</li><li>Ren, Y., 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=Increased+apoptotic+neutrophils+and+macrophages+and+impaired+macrophage+phagocytic+clearance+of+apoptotic+neutrophils+in+systemic+lupus+erythematosus.">Increased apoptotic neutrophils and macrophages and impaired macrophage phagocytic clearance of apoptotic neutrophils in systemic lupus erythematosus.</a> Arthritis Rheum. 48 (10), 2888-2897 (2003).</li><li>Connelly, A. N., 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=Optimization+of+methods+for+the+accurate+characterization+of+whole+blood+neutrophils.">Optimization of methods for the accurate characterization of whole blood neutrophils.</a> Sci Rep. 12 (1), 3667 (2022).</li><li>Carmona-Rivera, C., Kaplan, M. J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Low-density+granulocytes+in+systemic+autoimmunity+and+autoinflammation.">Low-density granulocytes in systemic autoimmunity and autoinflammation.</a> Immunol Rev. 314 (1), 313-325 (2023).</li><li>Yennemadi, A. S., Keane, J., Leisching, G. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Mitochondrial+bioenergetic+changes+in+systemic+lupus+erythematosus+immune+cell+subsets:+Contributions+to+pathogenesis+and+clinical+applications.">Mitochondrial bioenergetic changes in systemic lupus erythematosus immune cell subsets: Contributions to pathogenesis and clinical applications.</a> Lupus. 32 (5), 603-611 (2023).</li><li>Futoh, Y., 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=Peripheral+low-density+granulocytes+after+colorectal+cancer+surgery+in+predicting+recurrence.">Peripheral low-density granulocytes after colorectal cancer surgery in predicting recurrence.</a> BJS Open. 7 (1), zrac154 (2023).</li><li>Dwivedi, 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=Emergence+of+dysfunctional+neutrophils+with+a+defect+in+arginase-1+release+in+severe+COVID-19.">Emergence of dysfunctional neutrophils with a defect in arginase-1 release in severe COVID-19.</a> JCI Insight. 9 (17), e171659 (2024).</li></ol>

The authors have no disclosures.

Here, we present an optimized method of splitting the total neutrophil population into low- density and normal-density neutrophils, together with phenotypic characterization of each cell type using flow cytometry adapted from previous methods5.
This protocol is based on the isolation of LDNs and NDNs from whole blood. A crucial step is that total neutrophils are isolated through negative selection methods. Positive selection methods involve the use of antibodies that bind to surface markers, potentially activating the neutrophils and triggering degranulation5. This activation can interfere with downstream experiments by altering the functional and metabolic state of the neutrophils, leading to inaccurate results and skewing the interpretation of experimental outcomes. Therefore, negative selection ensures the isolation of neutrophils without inducing activation or functional changes. Additionally, the use of negative separation-based magnetic isolation eliminates the need for red blood cell (RBC) lysis. This not only reduces extra wash steps and cell death, thus preserving yield, but it also increases the purity of the isolated neutrophils by minimizing RBC contamination. In comparison to the original protocol, a cell separation buffer was used throughout the entire process, including washing and resuspension, in place of PBS. This contains additives that reduce cell clumping and minimize non-specific binding during magnetic isolation. By using cell separation buffer consistently, we achieved improved cell separation efficiency, higher purity, and a greater yield of viable, untouched neutrophils compared to using PBS. This resulted in enhanced precision for downstream analyses. Additionally, the density gradient was performed over multiple tubes rather than over a single tube to improve the resolution between the two cell types.
The successful separation of the two neutrophil subtypes is unsurprisingly highly dependent on the precise formulation and accurate layering of each gradient15. Equally important is the layering of the 70% over the 81%, as well as the neutrophil suspension (in 55%) over the 70% layer. We highly recommend practicing this method. It is best to use a transfer pipette when layering and positioning the 15 mL tube almost parallel to the bottom of the biosafety cabinet. Mixing of the gradients, even slightly, will cause indistinct and diffuse bands, which may render indistinct populations. Care should be taken to slowly remove only the neutrophil bands using a Pasteur pipette, as the layers above and below should not be aspirated, if possible, due to their toxicity. It is important to minimize contamination of the neutrophil fraction with the Isotonic working solution to avoid any adverse effects on the cells15. Finally, higher cell numbers can result in an overall higher density of the LDN and NDN bands, resulting in poorer resolution of the cell populations. We, therefore, recommend performing a total neutrophil count prior to resuspension in the 55% solution. This is particularly significant if using &#62;12 mL whole blood for neutrophil isolation or if the total neutrophil count exceeds 5-6&#160;&#215; 106.
Alternatives to this method consist of the dextran/Percoll combination, which does not rely on magnetic separation and is essentially a single-step protocol16. The use of dextran sedimentation to remove erythrocytes may not be as efficient or consistent as other methods like direct RBC lysis or density gradients. Dextran sedimentation can leave residual RBCs in the supernatant, which could affect the purity of the neutrophil population. Without a negative selection step, there is a risk that neutrophils could be activated by residual antibodies or other stimuli, which might affect their behavior in downstream assays. The manual removal of PBMC and neutrophil layers from the density gradient medium could result in contamination between the cell populations, particularly if the separation is not clean.
This study presents a relatively simplistic flow cytometry panel to determine the purity of the isolated LDNs and NDNs and perform a minimal characterization of these cells. The markers used here are widely reported in the literature as part of multiple, more complex flow cytometry panels involving neutrophil research. We chose to condense the panel to determine isolation purity, percent frequency of live and dead cells, and examine neutrophil maturation status (based on CD10 and CD16 expression). However, it can be expanded to suit the needs of various end-users&#39; studies. This protocol was specifically designed to separate LDNs and NDNs for individual assessment, as distinguishing these subpopulations together on a flow cytometry panel has proven challenging due to their relative indistinctness (Figure 2H). Consistent with previous reports5, it was found that LDNs and NDNs from healthy individuals cannot be reliably differentiated when analyzed simultaneously. Therefore, isolating them beforehand allows for a more accurate and detailed characterization of each subpopulation.
We suggest that during the optimization phase for this protocol, end-users might choose to include basic lymphocyte markers such as CD3 and CD19 in their flow cytometry panel. This can help with troubleshooting, as suboptimal magnetic isolation can result in the inclusion of lymphocytes in the total neutrophil isolate, which could potentially carry forward into the LDN fraction owing to similar cellular densities. For the purposes of optimization, users may choose to add CD45 to better troubleshoot the contaminants in their isolated fractions, i.e., CD45-ve could be RBCs, and CD45+ve could indicate PBMC contamination. Neutrophil subpopulations were defined based on surface marker expression, which is a dynamic property and can present a high level of variability between donors. Thus, in keeping with good flow cytometry practices, using FMO controls is also suggested, as this can help reduce inter-donor variability and define clearer sub-populations.
We also acknowledge that this protocol was only optimized for fresh whole blood, in accordance with the guidelines from the magnetic isolation kit, which states that only unprocessed, whole blood should be used with this kit and that recovery of the desired isolated cells decreases with samples that are &#62;24 h old. This eliminates the options for the starting material from which neutrophils can be isolated, such as bronchoalveolar lavage fluid (BALF), pleural fluid, ascites, etc. Connelly et al. have shown that delays in processing neutrophils17, even from fresh-drawn whole blood, can alter their phenotype and surface expression. In keeping with this, we recommend the commencement of processing with as little delay as possible from the time of the blood draw. So, while this protocol is ideal for fresh whole blood, compared to single-step protocols like the dextran/Percoll, it can be a relatively long and time-consuming method that does not offer an intermediate stop point. This presents a limitation in cases of clinical studies where samples may be received at later hours in the day. Additionally, this method does not permit the sorting of LDN and NDN subsets, as methods for sorting subsets (by flow cytometry or otherwise) run the risk of unintentionally activating neutrophils.
Neutrophil subpopulations have garnered significant attention in conditions such as systemic lupus erythematosus (SLE)18,19, cancer20, and COVID-1921. The growing interest in these cell types, particularly in the context of inflammatory and autoimmune diseases, underscores the need for reliable methods to accurately assess each population and better understand their individual contributions to pathogenesis.

Neutrophils are granular immune cells and the most abundant leukocyte in peripheral blood, constituting about 50%-70% of leukocytes on average. They develop in the bone marrow from granulocyte-monocyte precursors (GMPs), which in turn develop from hematopoietic progenitor cells (HPCs) in the presence of granulocyte colony-stimulating factor (G-CSF). At homeostasis, they have a lifespan of ~24 h, but studies have shown that their lifespan can be extended under specific physiological conditions and their associated microenvironments such as chronic immune activation1, inflammation1, and even tissue residency in steady state2. Neutrophils have long been considered the first line of defense against pathogens and elicit their anti-microbial effects through 3 major effector functions -- degranulation, phagocytosis, and neutrophil extracellular trap (NET) activation and release (NETosis).
Most studies on neutrophil function and biology examine outcomes for the total neutrophil population. However, from studies in cancer settings delineating N1 (anti-tumor)/ N2 (pro-tumor) subtypes to the classification of neutrophils based on maturity, disease, and physiological state, and even cellular density (low density and normal density neutrophils), it has become increasingly apparent that the human neutrophil population constitutes phenotypically diverse subtypes. Whether the existence of these neutrophil subtypes can be attributed to being completely distinct cell types or due to the complex nature of plasticity, there exists a growing body of literature on atypical neutrophils and presents a compelling opportunity to study low-density neutrophils separate from normal-density neutrophils3.
Described for the first time in SLE patients as a pro-inflammatory neutrophil subset4, LDNs have since been identified in chronic diseases, pregnancy, and even in healthy circulation, in pro-inflammatory as well as suppressive capacities5,6,7,8. LDNs are found concurrently with peripheral blood mononuclear cells (PBMCs) when whole blood is centrifuged over density gradient media. Their specific density corresponds to approximately 1.077 g/mL, compared to NDNs at 1.083 g/mL9. While there is still considerable debate on the subject, there exists speculation that LDNs resemble a more immature granulocyte phenotype (similar to promyelocytes and myelocytes, with a density below 1.080 g/mL)9,10. Others still speculate that there are both mature and immature LDN phenotypes depending on the presence or absence of disease11,12,13. Nevertheless, LDNs have also been detected in healthy individuals; however, their inclusion in some studies is limited due to the difficulty in isolating them in sufficient numbers5.
This study aimed to isolate these two populations in quantities that would allow us to perform downstream in situ metabolic experiments (minimum 0.5&#160;&#215; 106 cells/mL). In doing so, an existing protocol5 was optimized with commonly reported phenotypic markers13,14 that provide the best outcome for isolating and characterizing LDNs and NDNs from whole blood (Figure 1A).

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>14 mL Polypropylene Round-Bottom Tube (17 x 100 mm)</td>
			<td>Corning Science</td>
			<td>352059</td>
			<td></td>
		</tr>
		<tr>
			<td>APC anti-human CD14 (63D3)</td>
			<td>BioLegend</td>
			<td>367118</td>
			<td></td>
		</tr>
		<tr>
			<td>Brilliant Violet 421 anti-human CD10 (25 tests)</td>
			<td>BioLegend</td>
			<td>312217</td>
			<td></td>
		</tr>
		<tr>
			<td>Dulbecco&#39;s Phosphate-Buffered Saline</td>
			<td>Sigma</td>
			<td>D8537-1L</td>
			<td></td>
		</tr>
		<tr>
			<td>EasyEights EasySep Magnet</td>
			<td>StemCell Technologies</td>
			<td>#18103</td>
			<td></td>
		</tr>
		<tr>
			<td>EasySep Buffer (cell separation buffer)</td>
			<td>StemCell Technologies</td>
			<td>#20144</td>
			<td></td>
		</tr>
		<tr>
			<td>EasySep Direct Human Neutrophil Isolation Kit</td>
			<td>StemCell Technologies</td>
			<td>#19666</td>
			<td></td>
		</tr>
		<tr>
			<td>FcR Blocking Reagent, human</td>
			<td>Miltenyi Biotec</td>
			<td>130-059-901</td>
			<td></td>
		</tr>
		<tr>
			<td>FITC anti-human CD16 (3G8)</td>
			<td>BioLegend</td>
			<td>302005</td>
			<td></td>
		</tr>
		<tr>
			<td>OneComp eBeads Compensation Beads</td>
			<td>eBioscience Inc.</td>
			<td>01-1111-42</td>
			<td></td>
		</tr>
		<tr>
			<td>PE/Cy7 anti-human CD86 (BU63)</td>
			<td>BioLegend</td>
			<td>374209</td>
			<td></td>
		</tr>
		<tr>
			<td>PE/Dazzle 594 anti-human CD15 (SSEA-1)</td>
			<td>BioLegend</td>
			<td>323037</td>
			<td></td>
		</tr>
		<tr>
			<td>Phosphate-Buffered Saline Tablets&#160;</td>
			<td>Gibco</td>
			<td>18912-014</td>
			<td></td>
		</tr>
		<tr>
			<td>Zombie NIR Fixable Viability Kit</td>
			<td>BioLegend</td>
			<td>423105</td>
			<td></td>
		</tr>
	</tbody>
</table>

the isolation and characterization of low- and normal- density neutrophils from whole blood

Emerging research shows that the circulating neutrophil population in humans consists of diverse subtypes and should not be studied as a single population, as has been done historically. In particular, low-density and normal-density neutrophils (LDNs, NDNs) have been shown to have functionally and metabolically distinct profiles, a factor that must be considered when publishing neutrophil research. Here, we present a modified method for the untouched isolation and separation of LDNs and NDNs from whole blood.
The density gradient medium (1.135 g/mL) is combined at 9:10 with 10x PBS. Specific density gradients of 55%, 70%, and 81% are subsequently made by combining the 100% density gradient medium with 1x phosphate-buffered saline (PBS). Neutrophils isolated from 12 mL of peripheral whole blood obtained from consented donors using a negative selection-based magnetic isolation kit are resuspended in the 55% fraction. A volume of 3 mL of the 81% and 70% fractions is layered into a 15 mL tube, followed by the 55% fraction containing total neutrophils. The density gradients are then centrifuged at 720 x&#160;g for 30 min. Two distinct bands are obtained at the 55%/70% interface (LDNs) and 70%/81% interface (NDNs). The cells are carefully pipetted into separate tubes and washed using PBS. The purity of the isolated fractions is determined using flow cytometry. Both LDNs and NDNs were defined as CD14lo CD15+ SSChi by flow cytometry. Isolation purity was calculated at &#8805;93% of viable cells for both types.
This method provides a reliable and efficient approach for separating LDN and NDNs from peripheral blood, ensuring high purity and viability of the isolated cells. Enhancing the precision of neutrophil isolation facilitates more accurate downstream analyses of these distinct neutrophil subpopulations. These are critical for advancing our understanding of neutrophil heterogeneity and its implications in various physiological and pathological contexts.

The successful layering of total neutrophils over the density gradient medium can be observed in Figure 1B. Two distinct bands should be obtained. If mixing of the gradients occurs, or the number of total neutrophils layered per tube is high (greater than roughly 5-6&#160;&#215; 106), the bands will look diffuse (Figure 1C), and the risk of the two neutrophil subtypes mixing increases significantly. To avoid the latter, we recommend layering up to 5-6 &#215; 106 total neutrophils per density-gradient tube. Despite reports of LDNs being at very low numbers in healthy individuals, which therefore makes them unattainable for downstream studies, this method shows good yield of both LDNs (mean 3.28&#160;&#215; 106 cells/mL) and NDNs (mean 10.64&#160;&#215; 106 cells/mL) and purity from healthy participants (Figure 2).
The average isolation purity for LDNs was 93.80% (&#177; 5.80), and for NDNs, it was 96.30% (&#177; 3.30; Figure 2A) after the isolation procedure, with minimal contamination of other cell types (Figure 2B). DAPI staining of nuclei confirmed LDN/NDN presence through nuclei morphology and showed distinctive multi-lobed nuclei in NDNs after isolation (Figure 2C). Absolute counts after isolation showed a common trend of more NDNs being present than LDNs, with mean yields of 10.64&#160;&#215; 106 cells/mL and 3.28&#160;&#215; 106 cells/mL, respectively (Figure 2D). Using flow cytometry, both LDNs and NDNs were defined as CD14lo CD86- CD15+ SSChi cells13 (Figure 2E). CD14 is a common myeloid marker, CD15 is a neutrophil identification marker, and CD10 and CD16 are commonly described neutrophil markers of maturity and activation13. Fluorescence-minus-one controls (FMOs) were used to distinguish CD16 and CD10 positive populations from negative populations. A largely singular population of mature LDNs as well as NDNs (CD16hiCD10+) were observed in healthy individuals, which is consistent with reports in the literature13, as healthy individuals are not likely to have a high percentage of immature neutrophils (CD16lo/intCD10+) in circulation (Figure 2F,G). On average, the frequency of CD16hiCD10+ LDNs was 93.33% (&#177; 5.29), CD16hiCD10+ NDNs was 98.03% (&#177; 1.40), CD16lo/intCD10+ was 0.49% (&#177; 0.38), and CD16lo/intCD10+ was0.17% (&#177; 0.06; Figure 2F,G). When CD16+CD10+ populations were superimposed upon each other, the degree of overlap indicated no noticeable differences in the expression of these markers in LDNs compared to NDNs (Figure 2H). The cells were acquired using a flow cytometer and all data analysis was performed using the appropriate software for flow cytometry.
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/67805/67805fig01.jpg" /> 
Figure 1:&#160;Overview of the protocol. (A) A two-step isolation protocol of LDNs and NDNs from whole blood. The first step consists of total neutrophils isolated from whole blood using negative selection. The second step involves resuspending the total neutrophils in 55% Isotonic working solution and layering it on top of an 81% and 70% gradient. After centrifugations, LDNs will be at the interface of the 55% and 70% layers and NDNs at the interface of the 81% and 70% layers. (B) Visual representation of ideally separated LDNs and NDNs after gradient medium centrifugation. (C) Suboptimal separation of LDNs and NDNs as seen by the diffuse nature of the bands. There is a high likelihood in this case that NDNs contaminate the LDN fraction or vice versa.&#160;Graphic created in BioRender. Yennemadi, A. (2025)&#160; https://BioRender.com/t03m122.&#160;<a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/67805/67805fig01large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/67805/67805fig02.jpg" /> 
Figure 2: Representative results of the protocol. (A) Percent isolation purity of LDNs and NDNs from whole blood. (B) Percentage of contaminating cells (B cells, T cells, and monocytes) after isolation. (C) DAPI staining of LDNs and NDNs after isolation showing multi-lobed nuclei in NDNs and single-lobed nuclei in LDNs. (D) Absolute number of LDNs and matched NDNs isolated from whole blood. (E) Gating strategy used to define LDNs and NDNs, determine their purity, and calculate their frequency. Debris, doublets, and dead cells were eliminated from analysis (top row), and CD86- CD14lo, CD15+ SSChi cells were gated upon to define neutrophils. (F,G) CD16 and CD10 expression were used to define subpopulations in conjunction with the use of fluorescence-minus-one controls. Frequency of isolated mature (CD16hiCD10+) and immature (CD16lo/intCD10+) LDN and NDN subpopulations, reported as the percentage of total LDNs and NDNs (defined as CD15+SSChi cells). (H) Dot plot showing CD16+ CD10+ LDNs superimposed over CD16+ CD10+ NDNs in healthy individuals. Mean &#177; SD, Paired t-test, n = 3-8. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/67805/67805fig02large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Here, we provide a reliable approach for isolating low- and normal-density neutrophils from whole blood using magnetic isolation (negative selection) and discontinuous density gradient medium. It ensures untouched isolation of high-purity cells (&#8805;93%), facilitating accurate downstream analysis of neutrophil subpopulations, crucial for understanding their roles in health and disease.

The Isolation and Characterization of Low- and Normal- Density Neutrophils from Whole Blood

Emerging research shows that the circulating neutrophil population in humans consists of diverse subtypes and should not be studied as a single ...

the-isolation-characterization-low-normal-density-neutrophils-from

Nanyang Technological University

Research

JoVE Journal

Immunology and Infection

348 Views.  The University of Dublin. Here, we provide a reliable approach for isolating low- and normal-density neutrophils from whole blood using magnetic isolation (negative selection) and discontinuous density gradient medium. It ensures untouched isolation of high-purity cells (≥93%), facilitating accurate downstream analysis of neutrophil subpopulations, crucial for understanding their roles in health and disease.

Video: The Isolation and Characterization of Low- and Normal- Density Neutrophils from Whole Blood

Isolation of Mouse Peritoneal Cavity Cells

The peritoneal cavity is a membrane-bound and fluid-filled abdominal cavity of mammals, which contains the liver, spleen, most of the gastro-intestinal tract and other viscera. It harbors a number of immune cells including macrophages, B cells and T cells. The presence of a high number of na&iuml;ve macrophages in the peritoneal cavity makes it a preferred site for the collection of na&iuml;ve tissue resident macrophages (1). The peritoneal cavity is also important to the study of B cells because of the presence of a unique peritoneal cavity-resident B cell subset known as B1 cells in addition to conventional B2 cells. B1 cells are subdivided into B1a and B1b cells, which can be distinguished by the surface expression of CD11b and CD5. B1 cells are an important source of natural IgM providing early protection from a variety of pathogens (2-4). These cells are autoreactive in nature (5), but how they are controlled to prevent autoimmunity is still not understood completely. On the contrary, CD5+ B1a cells possess some regulatory properties by virtue of their IL-10 producing capacity (6). Therefore, peritoneal cavity B1 cells are an interesting cell population to study because of their diverse function and many unaddressed questions associated with their development and regulation. The isolation of peritoneal cavity resident immune cells is tricky because of the lack of a defined structure inside the peritoneal cavity. Our protocol will describe a procedure for obtaining viable immune cells from the peritoneal cavity of mice, which then can be used for phenotypic analysis by flow cytometry and for different biochemical and immunological assays.

The peritoneal cavity in mammals contains different immune cell populations crucial for innate immune responses. An efficient isolation method is required for biochemical and functional analyses of these cells. Here we provide a comprehensive method for the isolation of peritoneal cavity cells in the mouse.

The peritoneal cavity is a membrane-bound and fluid-filled abdominal cavity of mammals, which contains the liver, spleen, most of the gastro-intestinal ...

A Functional Whole Blood Assay to Measure Viability of Mycobacteria, using Reporter-Gene Tagged BCG or M.Tb (BCG lux/M.Tb lux)

Functional assays have long played a key role in measuring of immunogenicity of a given vaccine. This is conventionally expressed as serum bactericidal titers. Studies of serum bactericidal titers in response to childhood vaccines have enabled us to develop and validate cut-off levels for protective immune responses and such cut-offs are in routine use. No such assays have been taken forward into the routine assessment of vaccines that induce primarily cell-mediated immunity in the form of effector T cell responses, such as TB vaccines. In the animal model, the performance of a given vaccine candidate is routinely evaluated in standardized bactericidal assays, and all current novel TB-vaccine candidates have been subjected to this step in their evaluation prior to phase 1 human trials. The assessment of immunogenicity and therefore likelihood of protective efficacy of novel anti-TB vaccines should ideally undergo a similar step-wise evaluation in the human models now, including measurements in bactericidal assays.
Bactericidal assays in the context of tuberculosis vaccine research are already well established in the animal models, where they are applied to screen potentially promising vaccine candidates. Reduction of bacterial load in various organs functions as the main read-out of immunogenicity. However, no such assays have been incorporated into clinical trials for novel anti-TB vaccines to date.
Although there is still uncertainty about the exact mechanisms that lead to killing of mycobacteria inside human macrophages, the interaction of macrophages and T cells with mycobacteria is clearly required. The assay described in this paper represents a novel generation of bactericidal assays that enables studies of such key cellular components with all other cellular and humoral factors present in whole blood without making assumptions about their relative individual contribution. The assay described by our group uses small volumes of whole blood and has already been employed in studies of adults and children in TB-endemic settings. We have shown immunogenicity of the BCG vaccine, increased growth of mycobacteria in HIV-positive patients, as well as the effect of anti-retroviral therapy and Vitamin D on mycobacterial survival in vitro. Here we summarise the methodology, and present our reproducibility data using this relatively simple, low-cost and field-friendly model.
Note: Definitions/Abbreviations
BCG lux = M. bovis BCG, Montreal strain, transformed with shuttle plasmid pSMT1 carrying the luxAB genes from Vibrio harveyi, under the control of the mycobacterial GroEL (hsp60) promoter. 
CFU = Colony Forming Unit (a measure of mycobacterial viability).

A Functional Whole Blood Assay to Measure Viability of Mycobacteria, using Reporter-Gene Tagged BCG or M.Tb BCG lux/M.Tb lux

We describe an alternative approach to the enumeration of mycobacteria in vitro, which uses reporter-gene tagged mycobacteria instead of colony-forming units (CFU). &#x201C;Survival&#x201D; of organisms as well as host response-markers are measured simultaneously, providing a low-cost, versatile and functional system for studies of host/pathogen interactions in the context of tuberculosis.

Functional assays have long played a key role in measuring of immunogenicity of a given vaccine. This is conventionally expressed as serum bactericidal ...

Isolation and Characterization of Dendritic Cells and Macrophages from the Mouse Intestine

Within the intestine reside unique populations of innate and adaptive immune cells that are involved in promoting tolerance towards commensal flora and food antigens while concomitantly remaining poised to mount inflammatory responses toward invasive pathogens1,2. Antigen presenting cells, particularly DCs and macrophages, play critical roles in maintaining intestinal immune homeostasis via their ability to sense and appropriately respond to the microbiota3-14. Efficient isolation of intestinal DCs and macrophages is a critical step in characterizing the phenotype and function of these cells. While many effective methods of isolating intestinal immune cells, including DCs and macrophages, have been described6,10,15-24, many rely upon long digestions times that may negatively influence cell surface antigen expression, cell viability, and/or cell yield. Here, we detail a methodology for the rapid isolation of large numbers of viable, intestinal DCs and macrophages. Phenotypic characterization of intestinal DCs and macrophages is carried out by directly staining isolated intestinal cells with specific fluorescence-labeled monoclonal antibodies for multi-color flow cytometric analysis. Furthermore, highly pure DC and macrophage populations are isolated for functional studies utilizing CD11c and CD11b magnetic-activated cell sorting beads followed by cell sorting.

Here, we detail a methodology for the rapid isolation of mouse intestinal dendritic cells (DCs) and macrophages. Phenotypic characterization of intestinal DCs and macrophages is performed using multi-color flow cytometric analysis while magnetic bead enrichment followed by cell sorting is used to yield highly pure populations for functional studies.

Within the intestine reside unique populations of innate and adaptive immune cells that are involved in promoting tolerance towards commensal flora and ...

Isolation of Precursor B-cell Subsets from Umbilical Cord Blood

Umbilical cord blood is highly enriched for hematopoietic progenitor cells at different lineage commitment stages. We have developed a protocol for isolating precursor B-cells at four different stages of differentiation. Because genes are expressed and epigenetic modifications occur in a tissue specific manner, it is vital to discriminate between tissues and cell types in order to be able to identify alterations in the genome and the epigenome that may lead to the development of disease. This method can be adapted to any type of cell present in umbilical cord blood at any stage of differentiation.	
This method comprises 4 main steps. First, mononuclear cells are separated by density centrifugation. Second, B-cells are enriched using biotin conjugated antibodies that recognize and remove non B-cells from the mononuclear cells. Third the B-cells are fluorescently labeled with cell surface protein antibodies specific to individual stages of B-cell development. Finally, the fluorescently labeled cells are sorted and individual populations are recovered. The recovered cells are of sufficient quantity and quality to be utilized in downstream nucleic acid assays.

Here we describe a protocol for isolating subsets of precursor B-cells from umbilical cord blood. A sufficient quantity and quality of nucleic acids may be extracted from the cells and used in subsequent assays utilizing DNA or RNA.

Umbilical cord blood is highly enriched for hematopoietic progenitor cells at different lineage commitment stages. We have developed a protocol for ...

Isolation and Characterization of Neutrophils with Anti-Tumor Properties

Neutrophils, the most abundant of all white blood cells in the human circulation, play an important role in the host defense against invading microorganisms. In addition, neutrophils play a central role in the immune surveillance of tumor cells. They have the ability to recognize tumor cells and induce tumor cell death either through a cell contact-dependent mechanism involving hydrogen peroxide or through antibody-dependent cell-mediated cytotoxicity (ADCC). Neutrophils with anti-tumor activity can be isolated from peripheral blood of cancer patients and of tumor-bearing mice. These neutrophils are termed tumor-entrained neutrophils (TEN) to distinguish them from neutrophils of healthy subjects or na&#239;ve mice that show no significant tumor cytotoxic activity. Compared with other white blood cells, neutrophils show different buoyancy making it feasible to obtain a &#62; 98% pure neutrophil population when subjected to a density gradient. However, in addition to the normal high-density neutrophil population (HDN), in cancer patients, in tumor-bearing mice, as well as under chronic inflammatory conditions, distinct low-density neutrophil populations (LDN) appear in the circulation. LDN co-purify with the mononuclear fraction and can be separated from mononuclear cells using either positive or negative selection strategies. Once the purity of the isolated neutrophils is determined by flow cytometry, they can be used for in vitro and in vivo functional assays. We describe techniques for monitoring the anti-tumor activity of neutrophils, their ability to migrate and to produce reactive oxygen species, as well as monitoring their phagocytic capacity ex vivo. We further describe techniques to label the neutrophils for in vivo tracking, and to determine their anti-metastatic capacity in vivo. All these techniques are essential for understanding how to obtain and characterize neutrophils with anti-tumor function.

Neutrophils play an important role not only in host defense against invading microorganisms, but are also involved in the immune surveillance of tumor cells. Here, we describe techniques related to the isolation of neutrophils with anti-tumor properties and methods for monitoring anti-tumor neutrophil function in vitro and in vivo.

Neutrophils, the most abundant of all white blood cells in the human circulation, play an important role in the host defense against invading ...

Isolation of Viral Replication Compartment-enriched Sub-nuclear Fractions from Adenovirus-infected Normal Human Cells

During infection of human cells by adenovirus (Ad), the host cell nucleus is dramatically reorganized, leading to formation of nuclear microenvironments through the recruitment of viral and cellular proteins to sites occupied by the viral genome. These sites, called replication compartments (RC), can be considered viral-induced nuclear domains where the viral genome is localized and viral and cellular proteins that participate in replication, transcription and post-transcriptional processing are recruited. Moreover, cellular proteins involved in the antiviral response, such as tumor suppressor proteins, DNA damage response (DDR) components and innate immune response factors are also co-opted to RC. Although RC seem to play a crucial role to promote an efficient and productive replication cycle, a detailed analysis of their composition and associated activities has not been made. To facilitate the study of adenoviral RC and potentially those from other DNA viruses that replicate in the cell nucleus, we adapted a simple procedure based on velocity gradients to isolate Ad RC and established a cell-free system amenable to conduct morphological, functional and compositional studies of these virus-induced subnuclear structures, as well as to study their impact on host-cell interactions.

We provide a novel strategy to isolate viral replication compartments (RC) from adenovirus (Ad)-infected human cells. This approach represents a cell-free system that can help to elucidate the molecular mechanisms regulating viral genome replication and expression as well as regulation of viral-host interactions established at the RC.

During infection of human cells by adenovirus (Ad), the host cell nucleus is dramatically reorganized, leading to formation of nuclear microenvironments ...

Isolation, Characterization and Functional Examination of the Gingival Immune Cell Network

Immune cell networks in tissues play a vital role in mediating local immunity and maintaining tissue homeostasis, yet little is known of the resident immune cell populations in the oral mucosa and gingiva. We have established a technique for the isolation and study of immune cells from murine gingival tissues, an area of constant microbial exposure and a vulnerable site to a common inflammatory disease, periodontitis. Our protocol allows for a detailed phenotypic characterization of the immune cell populations resident in the gingiva, even at steady state. Our procedure also yields sufficient cells with high viability for use in functional studies, such as the assessment of cytokine secretion ex vivo. This combination of phenotypic and functional characterization of the gingival immune cell network should aid towards investigating the mechanisms involved in oral immunity and periodontal homeostasis, but will also advance our understanding of the mechanisms involved in local immunopathology.

We have established a technique for the isolation, phenotypic characterization and functional analysis of immune cells from murine gingiva.

Immune cell networks in tissues play a vital role in mediating local immunity and maintaining tissue homeostasis, yet little is known of the resident ...

Generation of Human Monocyte-derived Dendritic Cells from Whole Blood

Dendritic cells (DCs) recognize foreign structures of different pathogens, such as viruses, bacteria, and fungi, via a variety of pattern recognition receptors (PRRs) expressed on their cell surface and thereby activate and regulate immunity. 
The major function of DCs is the induction of adaptive immunity in the lymph nodes by presenting antigens via MHC I and MHC II molecules to na&#239;ve T lymphocytes. Therefore, DCs have to migrate from the periphery to the lymph nodes after the recognition of pathogens at the sites of infection. For in vitro experiments or DC vaccination strategies, monocyte-derived DCs are routinely used. These cells show similarities in physiology, morphology, and function to conventional myeloid dendritic cells. They are generated by interleukin 4 (IL-4) and granulocyte-macrophage colony-stimulating factor (GM-CSF) stimulation of monocytes isolated from healthy donors. Here, we demonstrate how monocytes are isolated and stimulated from anti-coagulated human blood after peripheral blood mononuclear cell (PBMC) enrichment by density gradient centrifugation. Human monocytes are differentiated into immature DCs and are ready for experimental procedures in a non-clinical setting after 5 days of incubation.

Here, we demonstrate how monocytes are isolated by magnetic bead separation from peripheral blood mononuclear cells after density gradient centrifugation of human anti-coagulated blood. Following incubation for 5 days, human monocytes are differentiated into immature dendritic cells and are ready for experimental procedures in a non-clinical setting.

Dendritic cells (DCs) recognize foreign structures of different pathogens, such as viruses, bacteria, and fungi, via a variety of pattern recognition ...

Dextran Enhances the Lentiviral Transduction Efficiency of Murine and Human Primary NK Cells

The efficient transduction of specific genes into natural killer (NK) cells has been a major challenge. Successful transductions are critical to defining the role of the gene of interest in the development, differentiation, and function of NK cells. Recent advances related to chimeric antigen receptors (CARs) in cancer immunotherapy accentuate the need for an efficient method to deliver exogenous genes to effector lymphocytes. The efficiencies of lentiviral-mediated gene transductions into primary human or mouse NK cells remain significantly low, which is a major limiting factor. Recent advances using cationic polymers, such as polybrene, show an improved gene transduction efficiency in T cells. However, these products failed to improve the transduction efficiencies of NK cells. This work shows that dextran, a branched glucan polysaccharide, significantly improves the transduction efficiency of human and mouse primary NK cells. This highly reproducible transduction methodology provides a competent tool for transducing human primary NK cells, which can vastly improve clinical gene delivery applications and thus NK cell-based cancer immunotherapy.

The goal of this study was to formulate technologies that allow for successful gene transduction in primary natural killer (NK) cells. The dextran-mediated lentiviral transduction of human or mouse primary NK cells results in higher gene expression efficiencies. This method of gene transduction will vastly improve NK cell genetic manipulation.

The efficient transduction of specific genes into natural killer (NK) cells has been a major challenge. Successful transductions are critical to defining ...

Isolation, Characterization, and Purification of Macrophages from Tissues Affected by Obesity-related Inflammation

Obesity promotes a chronic inflammatory state that is largely mediated by tissue-resident macrophages as well as monocyte-derived macrophages. Diet-induced obesity (DIO) is a valuable model in studying the role of macrophage heterogeneity; however, adequate macrophage isolations are difficult to acquire from inflamed tissues. In this protocol, we outline the isolation steps and necessary troubleshooting guidelines derived from our studies for obtaining a suitable population of tissue-resident macrophages from mice following 18 weeks of high-fat (HFD) or high-fat/high-cholesterol (HFHCD) diet intervention. This protocol focuses on three hallmark tissues studied in obesity and atherosclerosis including the liver, white adipose tissues (WAT), and the aorta. We highlight how dualistic usage of flow cytometry can achieve a new dimension of isolation and characterization of tissue-resident macrophages. A fundamental section of this protocol addresses the intricacies underlying tissue-specific enzymatic digestions and macrophage isolation, and subsequent cell-surface antibody staining for flow cytometric analysis. This protocol addresses existing complexities underlying fluorescent-activated cell sorting (FACS) and presents clarifications to these complexities so as to obtain broad range characterization from adequately sorted cell populations. Alternate enrichment methods are included for sorting cells, such as the dense liver, allowing for flexibility and time management when working with FACS. In brief, this protocol aids the researcher to evaluate macrophage heterogeneity from a multitude of inflamed tissues in a given study and provides insightful troubleshooting tips that have been successful for favorable cellular isolation and characterization of immune cells in DIO-mediated inflammation.

This protocol allows a researcher to isolate and characterize tissue-resident macrophages in various hallmark inflamed tissues extracted from diet-induced models of metabolic disorders.