We thank the Light Imaging Section in the Office of Science and Technology at the National Institute of Arthritis and Musculoskeletal and Skin Diseases of the National Institutes of Health. This research was supported by the Intramural Research Program of the National Institute of Arthritis and Musculoskeletal and Skin Diseases of the National Institutes of Health (ZIA AR041199).

Neutrophils from healthy human subjects were obtained after informed consent was provided under National Institutes of Health (NIH) Institutional Review Board (IRB) approved protocol. The protocol follows guidelines of NIH human research ethics committee.
1. Staining of the neutrophils and preparation of assay plate
<ol>
	<li>Take peripheral blood with appropriate written informed consent following the guideline of each institute and isolate neutrophils using any desired method. For example, the Ficoll-dextran method10,11 is a commonly used method for isolation of neutrophils from human peripheral blood. 
	NOTE: Although the method discussed here uses human neutrophils, mouse neutrophils may also be analyzed using a similar protocol.</li>
	<li>Resuspend neutrophils in Roswell Park Memorial Institute (RPMI; see Table of Materials) 1640 medium at 2.0 x 106 neutrophils/mL and place neutrophil suspension into 1.5 mL centrifuge tube. 
	NOTE: We usually do not add fetal bovine serum (FBS) to the culture media because albumin in FBS can reduce NET formation12 and heat-stable nuclease in FBS can degrade NETs13.</li>
	<li>Add membrane-permeable red DNA dye (see Table of Materials) at 1 &#181;L per 1.5 mL of neutrophil suspension.</li>
	<li>Incubate at room temperature for 5 min in the dark. Centrifuge at 2500 x g for 5 min at room temperature and remove supernatant.</li>
	<li>Resuspend neutrophils in 1 mL of RPMI, then centrifuge at 2500 x g for 5 min at room temperature and remove supernatant. Repeat 2x (wash total 3x).</li>
	<li>Resuspend neutrophils in 1 mL of RPMI and count using a cell counter. Dilute neutrophil suspension to 1.5 x 105 neutrophils/mL.</li>
	<li>Add 4 &#181;L of 1:100-pre-diluted membrane-impermeable green DNA dye (see Table of Materials) per 1 mL of neutrophil suspension.</li>
	<li>Put 100 &#181;L of neutrophil suspension per well into a clear tissue-culture treated 96-well plate (see Table of Materials). Set each condition in triplicate. 
	NOTE: We have previously shown7 that there is no difference in NET formation and quantification with this method if neutrophils are placed in plates with or without poly-L-lysine coating. Therefore, the use of tissue culture treated plate is sufficient for this method.</li>
	<li>Add 100 &#181;L of RPMI containing stimulus reagents with or without inhibitor, or any other reagent of interest in respective wells. Always use positive control wells by adding 500 nM phorbol 12-myristate 13-acetate (PMA) or 2.5 &#181;M calcium ionophore (A23187), 30 &#181;M AKT inhibitor was used here.</li>
	<li>Place plate in the live cell analysis system (see Table of Materials) that is housed in a 5% CO2 incubator. 
	NOTE: Condensation may appear on the top and bottom of the plate a few minutes after this step. This may inhibit proper imaging. Wipe and remove condensation thoroughly before the start of the scanning. Place the plate in the machine, start the software, input scanning protocol, and then wipe the plate just before the first scan.</li>
</ol>
2. Scanning plate to visualize NET-forming neutrophils
<ol>
	<li>Start the software (see Table of Materials for software details). Launch Add Vessel by pressing + at the top left corner.</li>
	<li>Choose Scan on Schedule. Choose New. 
	NOTE: Once this is created, run the same scanning protocol by choosing Copy Previous and selecting stored protocol on the next screen.</li>
	<li>Choose Standard. Set scan settings as: Cell-by-Cell options: None; Image channels: Phase, Green (Acquisition Time: 200 ms), Red (Acquisition Time: 400 ms); Objective: 20x.</li>
	<li>Choose the plate being used from the list. Select vessel location where to put the plate on the tray of the live cell imaging system.</li>
	<li>Select wells where samples are present and decide how many images to take per well. Based on the number of images per well, generate an estimated scan duration for the plate. Usually, 4 images per well is sufficient; however, this may vary depending on the conditions and frequency of scans.</li>
	<li>Input the information from each well (e.g., cell type and compound) by clicking Create Plate Map to provide a name for the study. 
	NOTE: The plate map can be prepared and saved in advance using the plate map editor in the software. The saved plate map data can be imported during this step. If desired, entering plate map information can be skipped and performed later. Data can also be obtained without entering information of plate layout. However, it is recommended to input plate information to make the subsequent analysis easier.</li>
	<li>On the next screen, select Basic Analyzer as the analysis type, and choose Analysis Protocol from drop-down list, which shows previously used analysis definitions (not scanning protocols). Spectral unmixing for both green and red can be left at 0.0 %. 
	NOTE: This step may be skipped, if desired.</li>
	<li>Schedule scan. For the experiment here, scan at every 15-20 min for 8 h . Set the starting time of the scan by dragging the white and gray bar on top of the screen. 
	NOTE: Avoid scanning too frequently, otherwise the machine may not work well due to overheating. Time of scanning should not exceed 12 h per 24 h. You may see an alert if scanning is too frequent.</li>
	<li>Check the scan setting on the next screen and press Add to Schedule to start scanning. Wait until the initial set of images are scanned to confirm if everything is working well.
	<ol>
		<li>Sometimes cells may not be properly focused. In that case, check if condensation is present (and wipe accordingly), plate is correctly set on the tray, or the position of the plate is correctly specified, etc. If cells are still floating and have not settled down to the bottom of the well, wait for about 5 min before scanning.</li>
	</ol>
	</li>
</ol>
3. Setting the analysis definition to quantify NETs
<ol>
	<li>Open the study (vessel) to be analyzed on View tab. Press Launch Analysis on the left of the screen. Choose Create New Analysis Definition.
	<ol>
		<li>If an analysis has been performed previously, use the same analysis definition with minor alterations by selecting Copy Existing Analysis Definition. In this case, go to step 3.3. If using the analysis without any alteration select Use Existing Analysis Definition; this is not recommended because the level of fluorescence may vary between assays on different days, and some minor corrections are usually necessary.</li>
	</ol>
	</li>
	<li>Select Basic Analyzer. Use all image channels: Phase, Green, Red, and Overlap. 
	NOTE: Although we usually use green and red object masks to count NETs, overlap object mask is useful when debris matters. In such cases, the number of overlap object count will be used as numerators instead of green object count (see step 3.9). If overlap object count is used instead of green object count, all red signals must be counted correctly. Adjust the setting of red signal to count all red objects with low red signal in images taken in later timepoints but not to count debris.</li>
	<li>Choose 6 - 8 representative sample images for training. For the experiment here, include the following images: 
	Images taken between 0 to 20 min to optimize the green signal setting to compensate for subtle green signals that can be generated in non-NET-forming neutrophils 
	Images of maximum NETs with positive control, taken between 3-6 h (time varies depending on the stimulation used) to optimize the green signal setting to define NET-forming neutrophils 
	Images taken around the 1 h timepoint to count the number of total cells (stained with red dye) since the nuclear red signal is the strongest around 1 h timepoint (when all the cells have settled to the bottom of the well) and gradually decreases due to cell death. 
	Images containing debris, to exclude them from being counted.</li>
	<li>Set the analysis definition. Red objects and green objects correspond with nuclei of all neutrophils and those that are forming NETs, respectively. Start with the following example of and press Preview Current or Preview All, and modulate each parameter to optimize results: 
	For Green: Segmentation- Background subtraction: Top-Hat; Radius: 100 &#181;M; Threshold: 0.3 GCU; Edge split: On; Edge sensitivity: -20; Cleanup -Hole fill: 100 &#181;m2; Adjust size 0 pixels; Filters- Area: min 20 &#181;m2, max 500 &#181;m2; Eccentricity: max 0.97; Mean Intensity: min 1.00 
	&#8203;For Red: Segmentation- Background subtraction: Top-Hat; Radius: 10 &#181;M; Threshold: 1.0 GCU; Edge split: ON; Edge sensitivity: -50; Cleanup-Hole fill: 50 &#181;m2; Adjust size 0 pixels; Filters- Area: min 20 &#181;m2, max 400 &#181;m2; Mean Intensity: min 1.5.
	<ol>
		<li>If excessive green signal appears in neutrophils which should not be forming NETs (e.g., unstimulated neutrophils at 0 min that have lobulated nuclei), it may be due to overflow of the red signal detected in the green channel. In such case, return to step 3.1, open Image Layers on the left of the screen, and remove the red signals from the green channel by using Spectral Unmixing.</li>
		<li>Another option is to set one well for single staining with nuclear red dye to clarify how much of the red signal should be removed from green channel. On the other hand, usually green signal bleeding into the red channel does not affect the analyses. 
		NOTE: It does not matter if the sensitivity to red signal is low and not all red signals are captured in the images that are taken at later timepoints (e.g., 6 h timepoint). The maximum number of red object count in each image is regarded as total number of neutrophils in the image and will be used as denominator at step 3.9. Usually, nuclear red signals peak around 1 h timepoint and gradually diminish due to cell death (Figure 1B). Therefore, adjust the setting of red signal to correctly count red objects in the images with maximum red signals.</li>
	</ol>
	</li>
	<li>Select scan times and wells to be analyzed. Usually, all time points and wells should be analyzed. Provide a label to the analysis definition.</li>
	<li>Check the summary and launch the analysis. It takes a few hours for completion of analysis (the duration depends on the number of timepoints and wells). Once launched, the name of the analysis definition will be shown under the name of the study in the View tab, and the complete date will be shown when it is done.</li>
	<li>After it is completed, open the analyzed study by double clicking the name of the analysis definition. Open Layers on the left of the screen and check if each cell is correctly marked. If it is not correctly marked, return to step 3.1 and repeat the subsequent steps.</li>
	<li>Click Graph Metrics on the left of the screen to export the data. Select Green Count, Red Count or Overlap Count (Per Image), and then choose the timepoints and wells to be exported. For select grouping, select Plate Map Replicates if all wells are correctly specified when scanning is done.</li>
	<li>Export the data. Calculate the percentage of NET-forming cells for each condition/timepoint by the following equation using an appropriate software. 
	<img alt="Equation 1" src="/files/ftp_upload/66051/66051eq01.jpg" style="margin: auto;" /> 
	NOTE: The reason why the denominator is maximum red object count is that the number of Red object peaks at around 1 h timepoint and gradually decreases due to the cell death.</li>
</ol>

Quantifying NET Formation Using Dual-Dye Live Cell Analysis

<ol>
	<li>Brinkmann, V., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Neutrophil+extracellular+traps+kill+bacteria.">Neutrophil extracellular traps kill bacteria.</a> Science. 303 (5663), 1532-1535 (2004).</li><li>Wigerblad, G., 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=Neutrophil+extracellular+traps+in+systemic+autoimmune+and+autoinflammatory+diseases.">Neutrophil extracellular traps in systemic autoimmune and autoinflammatory diseases.</a> Nat Rev Immunol. 23 (5), 274-288 (2022).</li><li>Wagner, D. D., Heger, L. A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Thromboinflammation:+From+atherosclerosis+to+COVID-19.">Thromboinflammation: From atherosclerosis to COVID-19.</a> Arterioscler Thromb Vasc Biol. 42 (9), 1103-1112 (2022).</li><li>Njeim, 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=NETosis+contributes+to+the+pathogenesis+of+diabetes+and+its+complications.">NETosis contributes to the pathogenesis of diabetes and its complications.</a> J Mol Endocrinol. 65 (4), R65-R76 (2020).</li><li>De Meo, M. L., Spicer, J. D. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=The+role+of+neutrophil+extracellular+traps+in+cancer+progression+and+metastasis.">The role of neutrophil extracellular traps in cancer progression and metastasis.</a> Semin Immunol. 57, 101595 (2021).</li><li>Nakabo, S., Romo-Tena, J., 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=Neutrophils+as+drivers+of+immune+dysregulation+in+autoimmune+diseases+with+skin+manifestations.">Neutrophils as drivers of immune dysregulation in autoimmune diseases with skin manifestations.</a> J Invest Dermatol. 142 (3 Pt B), 823-833 (2022).</li><li>Gupta, S., Chan, D. W., Zaal, K. J., 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=A+high-throughput+real-time+imaging+technique+to+quantify+NETosis+and+distinguish+mechanisms+of+cell+death+in+human+neutrophils.">A high-throughput real-time imaging technique to quantify NETosis and distinguish mechanisms of cell death in human neutrophils.</a> J Immunol. 200 (2), 869-879 (2018).</li><li>Nakabo, S., Kaplan, M. J., Gupta, S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Quantification+of+neutrophils+undergoing+NET+formation+and+distinguishing+mechanisms+of+neutrophil+cell+death+by+use+of+a+high-throughput+method.">Quantification of neutrophils undergoing NET formation and distinguishing mechanisms of neutrophil cell death by use of a high-throughput method.</a> Methods Mol Biol. 2543, 129-140 (2022).</li><li>Singh, 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=Moonlighting+chromatin:+when+DNA+escapes+nuclear+control.">Moonlighting chromatin: when DNA escapes nuclear control.</a> Cell Death Differ. 30 (4), 861-875 (2023).</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=Induction+and+quantification+of+NETosis.">Induction and quantification of NETosis.</a> Curr Protoc Immunol. 115, 14.41.11-14.41.14 (2016).</li><li>Hsu, A. Y., Peng, Z., Luo, H., Loison, F. <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+human+neutrophils+from+whole+blood+and+buffy+coats.">Isolation of human neutrophils from whole blood and buffy coats.</a> J Vis Exp. (175), 62837 (2021).</li><li>Neubert, 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=Serum+and+serum+albumin+inhibit+in+vitro+formation+of+neutrophil+extracellular+traps+(NETs).">Serum and serum albumin inhibit in vitro formation of neutrophil extracellular traps (NETs).</a> Front Immunol. 10, 12 (2019).</li><li>von Kockritz-Blickwede, M., Chow, O. A., Nizet, V. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Fetal+calf+serum+contains+heat-stable+nucleases+that+degrade+neutrophil+extracellular+traps.">Fetal calf serum contains heat-stable nucleases that degrade neutrophil extracellular traps.</a> Blood. 114 (25), 5245-5246 (2009).</li><li>Zhao, W., Fogg, D. K., 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=A+novel+image-based+quantitative+method+for+the+characterization+of+NETosis.">A novel image-based quantitative method for the characterization of NETosis.</a> J Immunol Methods. 423, 104-110 (2015).</li><li>Papayannopoulos, V. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Neutrophil+extracellular+traps+in+immunity+and+disease.">Neutrophil extracellular traps in immunity and disease.</a> Nat Rev Immunol. 18 (2), 134-147 (2018).</li></ol>

Authors have no competing financial interests.

Current methods to quantify NETs ex vivo have several drawbacks that limit our ability to study neutrophils, NETs, and potential therapeutic targets in an unbiased and high-throughput way10,14. For example, direct counting of NET-forming cells after immunofluorescent staining, considered the gold standard for quantification of NETs, is low-throughput and dependent on operator&#39;s subjective view. A plate assay detecting the fluorescence of membrane-imp...

Neutrophil extracellular traps (NETs) are web-like chromatin structures extruded from neutrophils in response to various inflammatory stimuli. NETs are composed of DNA, histones, and various anti-microbial proteins/peptides, which trap and kill infectious pathogens and invoke inflammatory responses1.
While NETs are beneficial for host defense against pathogens, they have gathered attention as a potential driver of various autoimmune diseases2, thrombosis3, metabolic diseases4, and metastatic growth of cancers5. As such, inhibition of NET formation is a potential therapeutic option for these diseases. However, despite some promising NETs-targeting molecules in development6, there is still no approved therapy that specifically affects this mechanism. This is, at least partially, attributable to the lack of objective, unbiased, reproducible, and high throughput quantification methods for NET formation.
We established and reported a new method utilizing a dual-color live-cell imaging platform7,8. Time-lapse images of neutrophils stained with membrane-permeable nuclear dye and membrane-impermeable DNA dye are analyzed by the software, and the numbers of pre- and post-NET-forming neutrophils are counted at multiple time points. Since the integrity of the plasma membrane is lost during NET formation by the regulation of PKC&#945;-mediated Lamin B and CDK4/6-mediated Lamin A/C disassembly9, NET-forming neutrophils are stained by membrane-impermeable DNA dye while healthy neutrophils are not. This method overcomes the problems of previously reported techniques to quantify NET formation and provides unbiased, high-throughput, reproducible, and accurate NET quantification in an automated manner.

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>AKT inhibitor</td>
			<td>Calbiochem</td>
			<td>124028</td>
			<td></td>
		</tr>
		<tr>
			<td>Clear 96-well plate</td>
			<td>Corning</td>
			<td>3596</td>
			<td></td>
		</tr>
		<tr>
			<td>Live cell analysis system</td>
			<td>Sartorius</td>
			<td>N/A</td>
			<td>Incucyte Software (v2019B)</td>
		</tr>
		<tr>
			<td>Membrane-impermeable DNA green dye&#160;</td>
			<td>Thermo Fisher Scientific</td>
			<td>S7020</td>
			<td></td>
		</tr>
		<tr>
			<td>Nuclear red dye</td>
			<td>Enzo</td>
			<td>ENZ-52406</td>
			<td>Neutrophil pellet becomes bluish after staining.</td>
		</tr>
		<tr>
			<td>RPMI</td>
			<td>Thermo Fisher Scientific</td>
			<td>11835030</td>
			<td>Phenol red containig RPMI can be used.</td>
		</tr>
	</tbody>
</table>

real-time high throughput technique to quantify neutrophil extracellular traps formation in human neutrophils

Neutrophils are myeloid-lineage cells that form a crucial part of the innate immune system. The past decade has revealed additional key roles that neutrophils play in the pathogenesis of cancer, autoimmune diseases, and various acute and chronic inflammatory conditions by contributing to the initiation and perpetuation of immune dysregulation through multiple mechanisms, including the formation of neutrophil extracellular traps (NETs), which are structures crucial in antimicrobial defense. Limitations in techniques to quantify NET formation in an unbiased, reproducible, and efficient way have restricted our ability to further understand the role of neutrophils in health and diseases. We describe an automated, real-time, high-throughput method to quantify neutrophils undergoing NET formation using a live cell imaging platform coupled with a membrane permeability-dependent dual-dye approach using two different DNA dyes to image intracellular and extracellular DNA. This methodology is able to help assess neutrophil physiology and test molecules that can target NET formation.

Author Spotlight: Quantifying Neutrophil Extracellular Traps in Disease and Drug Screening Using Dual-Color Live-Cell Imaging

Real-Time High Throughput Technique to Quantify Neutrophil Extracellular Traps Formation in Human Neutrophils

Our research focuses on neutrophils, which are essential first responders in the immune system and play a significant role in various diseases. Over the past two decades, it has become clear that neutrophils contribute to the development of cancer, autoimmune diseases, and other inflammatory conditions by disrupting immunoregulation. This includes forming neutrophilic extracellular traps, nets, web-like structures that respond to inflammation and could be targeted for therapy in these diseases.However, despite some promising molecules targeting nets, in development there is still no approved therapy that specifically affects this mechanism. This is at least partially attributable to the lack of an objective, unbiased, reproducible, and high-throughput quantification method for net formation. Our protocol employs dual-color live cell imaging to analyze neutrophil behavior using membrane permeable and impermeable dyes for precise net formation tracking.This method distinguishes between net-forming and healthy neutrophils based on membrane integrity and provides clear differentiation of cell death types through morphological changes absorbed in phase contrast imaging. This method overcomes the problems of previously-reported techniques to quantify net formation and provides an efficient, reproducible, and accurate net quantification in an automated manner. This method will help in neutrophil-targeted drug development by giving the ability to screen multiple therapeutic targets against net formation in a high-throughput manner.

This method provides phase contrast, red fluorescent (membrane-permeable dye) and green fluorescent (membrane-impermeable dye) images taken at each timepoint. Along with the NET-forming process, morphological changes are observed in phase contrast and red fluorescent images, and once the membrane is breached, green fluorescence can be observed (Figure 1). In this assay, NET-forming neutrophils are generally round, instead of forming web-like structure. This is because the resolution of the m...

Watch this Scientific Journal Video about Author Spotlight: Quantifying Neutrophil Extracellular Traps in Disease and Drug Screening Using Dual-Color Live-Cell Imaging at JoVE.com

We present an automated high-throughput method to quantify neutrophil extracellular traps (NETs) utilizing the live cell analysis system, coupled with a membrane permeability-dependent dual-dye approach.

Neutrophils are myeloid-lineage cells that form a crucial part of the innate immune system. The past decade has revealed additional key roles that ...

real-time-high-throughput-technique-to-quantify-neutrophil

Research

JoVE Journal

Immunology and Infection

Human Neutrophil Staining and Preparation of Neutrophil Assay Plate for Live Cell Analysis

After isolating neutrophils from human peripheral blood, resuspend them in RPMI 1640 Medium in a 1.5 milliliter centrifuge tube. Add one microliter of membrane permeable red DNA die to 1.5 milliliters of neutrophil suspension and incubate in the dark for five minutes. Centrifuge the neutrophil suspension at 2, 500g for five minutes at room temperature.After centrifugation, remove the tube containing pelleted neutrophils and aspirate the supernatant. Resuspend the neutrophils in one milliliter of RPMI and centrifuge it again. After the last wash, resuspend the neutrophils in one milliliter of RPMI.Add a small volume of neutrophil suspension to the hemocytometer and count them under a microscope. Dilute the neutrophil suspension to 1.5 times 10 to the fifth neutrophils per milliliter using RPMI. Add four microliters of one to 100 pre-diluted membrane impermeable green DNA dye to the one milliliter of neutrophil suspension.Dispense 100 microliters of neutrophil suspension per well into a clear tissue culture treated 96 well plate. Add 100 microliters of RPMI containing stimulus reagents with or without inhibitor into the respective wells. Place the plate in a live cell analysis system housed in a 5%carbon dioxide incubator.

Scanning Plate Setup and Quantitative Analysis of Neutrophil Extracellular Traps Formation in Human Neutrophils

To begin, start the live cell analysis system software. Press the plus symbol at the top left corner of the screen to initiate the add vessel. Choose Scan on Schedule, then select New to run the scanning program.Select Standard. Then set scan settings as cell-by-cell options to None and image channels to Phase, Green, and Red, with respective acquisition times. Set objective to 20x.From the list, choose the plate and select the vessel location to put the plate on the tray of the imaging system. Select the wells containing samples and decide the number of images to capture per well. This information automatically generates an estimated scan duration for the plate.Click Create Plate Map to input information for each well, such as cell type and compound. Then name the study. On the next screen, select Basic Analyzer as the analysis type and choose Analysis Definition from the dropdown list, which shows previously used analysis definitions.Leave spectral unmixing for both green and red at 0.0. Schedule the scan to occur every 15 to 20 minutes for eight hours. Drag the white and gray bar on top of the screen to set the starting time of the scan.On the next screen, review the scan settings, and press Add to Schedule to start scanning. After scanning, on the View tab, open the vessel for analysis. Press Launch Analysis on the left of the screen and select Create New Analysis Definition.Choose Basic Analyzer and use Phase, Green, Red, and Overlap image channels. Select six to eight representative sample images for training. To configure the analysis definition, set green objects to neutrophils forming neutrophil extracellular traps or NETs, and red objects to the nuclei of all neutrophils.Press Preview Current or Preview All and adjust each parameter to optimize the results. Choose the scan times and wells for analysis. Then provide a label for the analysis definition.Review the summary and launch the analysis. After analysis, double click on the name of the analysis definition to open the analyzed study. Open Layers on the left of the screen and check if each cell is correctly marked.Click Graph Metrics on the left of the screen, then select count per image for green count. Choose the time points and wells to be exported. For select grouping, select Plate Map Replicates to confirm all wells are correctly specified during scanning, and click on Export Data.Similarly, export the data for red count and overlap count. Using the given equation, calculate the percentage of NETs forming cells for each condition and time point. The time course of the NET formation is visualized by plotting the percentage of NET-forming neutrophils at each time point.Adding an AKT inhibitor blocked the NET formation in neutrophils stimulated with PMA or calcium ionophore. Demonstrating the potential molecules targeting NET formation may be tested in a high throughput manner using this methodology.

675 Views.  National Institutes of Health (NIH).  We present an automated high-throughput method to quantify neutrophil extracellular traps (NETs) utilizing the live cell analysis system, coupled with a membrane permeability-dependent dual-dye approach.

Quantifying NET Formation Using Dual-Dye Live Cell Analysis

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