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EoE Sub Articles

All procedures involving human participants have been performed in compliance with the institutional, national, and international guidelines for human welfare and have been reviewed by the local institutional review board.
1. Culture and Preparation of the THP-1 Monocyte Cell Line
<ol>
	<li>Culture THP-1 monocytes as a suspension culture in T25 flasks at 37 &#176;C + 5% CO2. Cells should be grown in 5 mL of Roswell Park Memorial Institute 1640 (RPMI 1640) + 10% Fetal Bovine Serum (FBS).</li>
	<li>Each day, suspend cells evenly throughout the growth media by gently shaking the flask, then immediately count cells with a hemocytometer. Cells should be passaged once cell density reaches 1 x 106 cells/mL:
	<ol>
		<li>Pre-warm RPMI 1640 + 10% FBS in a 37 &#176;C water bath.</li>
		<li>Transfer 2 x 105 cells into a 1.5 mL microcentrifuge tube or a 15 mL conical tube, and pellet cells by centrifuging at 500 x g at room temperature for 5 min.</li>
		<li>Remove the supernatant without disturbing the cell pellet and resuspend the pellet in 1 mL (1.5 mL microcentrifuge tube) or 5 mL (15 mL conical tube) of phosphate-buffered saline (PBS).</li>
		<li>Centrifuge the tube at 500 x g at room temperature for 5 min. Remove the PBS without disturbing the cell pellet.</li>
		<li>Resuspend the pellet in 1 mL of fresh RPMI 1640 + 10% FBS.</li>
		<li>Into a new T25 flask place 4 mL of warmed media, and to this add the resuspended cells from 1.2.5. Culture in a 37 &#176;C + 5% CO2 incubator until the cells require passaging (typically 3 days), or until cells are required for an experiment.</li>
	</ol>
	</li>
	<li>For an experiment with THP-1-derived macrophages, remove the required number of cells from the flask and plate prior to passaging:
	<ol>
		<li>Place the required number of 18 mm circular glass coverslips (#1.5 thickness) into the wells of a 12-well plate &#8212; typically 1 coverslip per condition and/or time point. Into each well aliquot 5 x 104 THP-1 monocytes. The number of cells added to each well can be altered if required.</li>
		<li>Bring up the total volume of each cell-containing well to 1 mL using RPMI + 10% FBS warmed to 37 &#176;C.</li>
		<li>Add 100 nM phorbol 12-myristate 13-acetate (PMA) to each well and culture for 3 days to induce differentiation of THP-1 monocytes into macrophage-like cells.</li>
	</ol>
	</li>
</ol>
2. Culture and Preparation of the J774.2 Macrophage Cell Line
<ol>
	<li>Culture J774.2 cells in T25 flasks at 37 &#176;C + 5% CO2. Cells should be grown in 5 mL of Dulbecco&#8217;s Modified Eagle Medium (DMEM) + 10% FBS and passaged once the culture reaches 80-90% confluency. To passage cells:
	<ol>
		<li>Remove all media from the flask and rise once with 5 mL of PBS.</li>
		<li>Remove PBS from the flask and replace with 5 mL of fresh DMEM + 10% FBS.</li>
		<li>Using a cell scraper, scrape the bottom of the flask to suspend the cells in the media. Vigorously pipette the cells several times to break up any cell aggregates.</li>
		<li>Dilute cells 1:5 by removing 4 mL of the cell suspension from the flask and replacing it with 4 mL of fresh media. The remaining cell suspension can be discarded, used to start a new cell culture in a fresh T25 flask, or used for an experiment.</li>
	</ol>
	</li>
	<li>To set up for an efferocytosis assay using J774.2 cells:
	<ol>
		<li>One day prior to the start of the experiment, suspend J774.2 cells into 5 mL of fresh media, as per steps 1.1.1&#8211;1.1.3. Count cells using a hemocytometer and prepare the necessary volume of cells at a concentration of 5 x 104 cells/mL.</li>
		<li>Place the necessary number of 18 mm circular glass coverslips (#1.5 thickness) into the wells of a 12-well plate. Into each well aliquot 1 mL of the 5 x 104 cells/mL cell suspension.</li>
		<li>Culture overnight to allow the cells to adhere to the coverslip and recover from passaging.</li>
	</ol>
	</li>
</ol>
3. Culture of Primary Human M2 Macrophages
<ol>
	<li>Collect 10 mL of heparinized human blood for every 12-well plate of M2 macrophages required.</li>
	<li>In a 15 mL centrifuge tube, layer 5 mL of human blood on top of 5 mL of pre-warmed Lympholyte-poly cell separation medium. Prepare multiple tubes if processing &#62;5 mL of blood rather than using larger volume tubes.</li>
	<li>Centrifuge at 300 x g for 35 min, using medium acceleration and no break.</li>
	<li>Carefully remove the upper mononuclear-cell-rich band using a plastic pipettor and transfer to a 50 mL centrifuge tube. If multiple tubes were prepared in step 3.2, the bands can be pooled into a single 50 mL tube. Bring volume of tube up to 50 mL with PBS.</li>
	<li>Centrifuge at 300 x g for 8 min and remove the supernatant. During this step place autoclaved 18 mm diameter circular coverslips (#1.5 thickness) into each well of a 12-well plate.</li>
	<li>Resuspend the cell pellet in 300 &#181;L of serum-free RPMI 1640 per desired number of wells; e.g., if 10 mL of blood was processed to prepare a full 12-well plate, suspend cell pellet in 3.6 mL of media.</li>
	<li>Add 300 &#181;L of the cell suspension to each coverslip-containing well in the 12-well plate. Incubate for 1 h at 37 &#176;C + 5% CO2.</li>
	<li>Gently wash coverslip 3x with 1 mL of warmed PBS to remove any non-adherent cells.</li>
	<li>Add 1 mL of RPMI 1640 + 10% FBS + 10 ng/mL recombinant human M-CSF + cell culture antibiotic/antimycotic. Incubate at 37 &#176;C + 5% CO2 for 5 days.</li>
	<li>Replace media with RPMI 1640 + 10% FBS + 10 ng/mL recombinant human M-CSF + 10 ng/mL recombinant human IL-4 + cell culture antibiotic/antimycotic. Incubate at 37 &#176;C + 5% CO2 for 2 days to complete M2 polarization.</li>
	<li>Polarized macrophages should be used within the next 3 days.</li>
</ol>
4. Preparation of Apoptotic Jurkat Cells
<ol>
	<li>Culture Jurkat cells in 5 mL of RPMI 1640 + 10% FBS at 37 &#176;C + 5% CO2. Jurkats are a suspension cell line and can be maintained by passaging 1:5 into fresh, pre-warmed media every 3&#8211;5 days.</li>
	<li>To prepare apoptotic cells, allow the Jurkat culture to grow to high density (4&#8211;5 days after passaging). Aliquot 1.5 mL into a 1.5 mL microcentrifuge tube and pellet cells by centrifugation at 500 x g for 5 min.</li>
	<li>Discard supernatant and re-suspend cell pellet in 1 mL of serum-free RPMI 1640 medium containing 1 &#181;M staurosporine.</li>
	<li>Incubate 16 h at 37 &#176;C + 5% CO2 to render cells apoptotic.</li>
	<li>If desired, confirm induction of apoptosis by staining with Annexin V:
	<ol>
		<li>Aliquot 100 &#181;L of staurosporine-treated Jurkat cell culture into a 1.5 mL microcentrifuge tube. Pellet cells by centrifugation at 500 x g for 5 min, discard supernatant, and re-suspend cell pellet in 100 &#181;L of serum-free RPMI 1640 medium.</li>
		<li>Add 1 &#181;L of fluorescein isothiocyanate (FITC)-conjugated Annexin V and incubate for 10 min at room temperature in the dark.</li>
		<li>Add 900 &#181;L of PBS and transfer the entire volume to a single well of a 12-well plate containing an 18 mm circular glass coverslip (#1.5 thickness). Spin down in a centrifuge equipped with a plate adaptor at 200 x g for 1 min to force cells to adhere to the coverslip. Alternatively, cells can be placed into a chambered slide for imaging.</li>
		<li>Image using a fluorescence microscope.</li>
	</ol>
	</li>
</ol>
5. Quantifying Efferocytic Uptake and Dynamics Using a Fixed Cell Efferocytosis Assay and Inside-out Staining
<ol>
	<li>Prepare THP-1, J774.2, or M2 human macrophages as described in Sections 1-3, respectively.</li>
	<li>The evening prior to the start of the experiment, prepare apoptotic Jurkat cells as described in Section 4.</li>
	<li>Immediately prior to the experiment, count apoptotic cells using a hemocytometer. Transfer sufficient numbers of apoptotic cells into a 1.5 mL microcentrifuge tube &#8211; we usually add 5 x 105 cells/well, providing a target:efferocyte ratio of 10:1.</li>
	<li>Pellet Jurkat cells by centrifugation at 500 x g for 5 min and resuspend in 500 &#956;L of PBS.</li>
	<li>During the centrifugation, aliquot 10 &#181;L of DMSO into a new 1.5 mL microcentrifuge tube. Dissolve into the DMSO a minimal amount of N-hydroxysuccinimidobiotin (NHS-Biotin). 5-10 crystals (~0.005 mg) is sufficient.</li>
	<li>Transfer the 500 &#956;L apoptotic cell/PBS suspension to the DMSO/NHS-biotin-containing tube. Then dilute a cell tracking dye to the manufacturer&#8217;s recommended concentration into the apoptotic cell suspension. Make certain to select a cell tracking dye that does not overlap spectrally with FITC-Streptavidin (e.g. red or far-red cell tracking dye).</li>
	<li>Incubate suspension for 20 min at room temperature in the dark. Add an equal volume of RPMI 1640 + 10% FBS and incubate for 5 min at room temperature in the dark to quench any unreacted dye.</li>
	<li>Pellet cells by centrifugation at 500 x g for 5 min, discard the supernatant, and re-suspend the stained apoptotic cells in 100 &#181;L of RPMI 1640 + 10% FBS per well of macrophages.</li>
	<li>Add 100 &#181;L of stained apoptotic cell suspension dropwise to each well of macrophages. Centrifuge 200 x g for 1 min in a centrifuge equipped with a plate adaptor to force contact between macrophages and apoptotic cells.</li>
	<li>Incubate plate for the desired period of time at 37 &#176;C + 5% CO2 in a tissue culture incubator. For macrophages, efferocytosed material is usually first detectable after 20&#8211;30 min, and is completed after 120&#8211;180 min.</li>
	<li>At the desired time point(s) remove cells from the incubator. Wash cells twice with 1 mL of room temperature PBS to stop efferocytosis and remove non-efferocytosed apoptotic cells.</li>
	<li>Add FITC-conjugated streptavidin at a 1:1,000 dilution to each well and incubate for 20 min in the dark. This will label the exposed biotin on any non-efferocytosed apoptotic cell material. 
	NOTE: If desired, cell nuclei can be stained during this step by the addition of 1:20,000 dilution of Hoechst 33342 or 4&#39;,6-Diamidino-2-Phenylindole, Dihydrochloride (DAPI).</li>
	<li>Wash cells 3 times with 1 mL PBS, gently shaking or rocking the samples for 5 min per rinse. Fix cells with 4% paraformaldehyde (PFA) in PBS for 20 min at room temperature. Rinse cells once with PBS to remove excess PFA.</li>
	<li>Mount coverslips on a slide for imaging and transfer to a fluorescence microscope. Capture z-stacks of a sufficient number of cells for accurate quantification &#8212; typically 10&#8211;30 cells per condition. Non-internalized apoptotic cell material will be apparent in the resulting image as cell-tracking dye-labeled material enveloped by FITC-streptavidin staining, while efferocytosed material forms discrete cell-tracking dye puncta free of any streptavidin staining.</li>
	<li>Quantify efferocytosis in the resulting images via a variety of measures:
	<ol>
		<li>Calculate the efferocytic index by determining the average number of discrete efferosomes (cell tracking dye+/streptavidin- puncta) per macrophage. Quantify only macrophages bound to an apoptotic cell or containing &#8805;1 visible efferosomes. Record macrophages bound to an apoptotic cell, but lacking discrete efferosomes, as having an efferocytic index of 0.</li>
		<li>Calculate efferocytic efficiency by measuring the fraction of macrophages that contain &#8805;1 efferosome.</li>
		<li>Calculate the rate of efferocytosis by imaging cells fixed and stained at multiple time points. Only image macrophages bound to apoptotic cells, or containing visible efferosomes, with z-stacks captured of each cell. Once imaged, determine the rate of efferocytosis:
		<ol>
			<li>Using the streptavidin staining as a guide, and the freehand or polygon selection tool in FIJI/ImageJ (or other image analysis software package), circle all of the cell tracking dye+/streptavidin- (e.g. internalized) material in a single plane of the z-stack. Measure the integrated intensity of the cell-tracking dye this region. Individual measures for each efferosome (e.g. diameter, positioning relative to the cell border or nucleus, etc.) can easily be acquired simultaneously with these measurements, greatly increasing the data collected during analysis.</li>
			<li>On the same z-section, using the streptavidin staining as a guide and the freehand or polygon selection tool, circle all of the cell tracking dye+/streptavidin+ (e.g. non-internalized) material in a single plane of the z-stack. Only include staining from apoptotic cells in contact with the phagocyte. Measure the integrated intensity of this region.</li>
			<li>Repeat steps 4.2.3.1 to 4.2.3.2 for the remaining z-sections of the image. Sum the integrated intensity of the efferocytosed (&#931;eff) and non-efferocytosed (&#931;ne) materials. The fraction of the apoptotic cell which has been efferocytosed can be calculated for the cell as: 
			<img alt="Equation 1" src="/files/ftp_upload/21236/21236_Equation1.jpg" style="margin: auto;" /></li>
			<li>Quantify the fraction efferocytosed for all cells at all time points. Note that the fluorescent intensity of apoptotic cells/efferosomes can vary between images due to variations in the uptake of cell tracking dyes by individual apoptotic cells, and due to changes in image acquisition parameters such as exposure time. As such, only compare normalized values such as Fraction Efferocytosed, or intensity-independent values such as efferocytic index and efferocytic efficiency, between images, between experimental conditions, and between repeat experiments.</li>
		</ol>
		</li>
		<li>To ensure the resulting dataset accurately reflects the variation in efferocytosis between cells, conduct these analyses on the maximum number of cells possible in each experiment. 
		NOTE: Efferocytic efficiency and efferocytic index can be rapidly calculated (a few seconds/cell), and we typically aim to analyze at least 100 cells per experiment, repeating each experiment at least 3 times. Calculating the fraction of efferocytosed material, and efferosome-specific measures are more laborious, typically taking 2&#8211;3 min/cell for an experienced analyst. For these calculations, we quantify a minimum of 15 cells per condition, per experiment.</li>
		<li>Record efferocytic index, fraction efferocytosed, and individual efferosome data on a per-cell basis. 
		NOTE: This allows for data analysis using single-cell approaches, thus allowing for inter-cell variations to be quantified. Population-level analyses can still be conducted on these datasets by averaging single-cell data acquired in individual experiments. Efferosome-specific measurements can be analyzed at the population level, single-cell level, and as ensembles (e.g. as populations of efferosomes independent of the cells containing them).</li>
	</ol>
	</li>
</ol>

<table><tbody><tr><td>RPMI 1640 Media</td><td>Wisent</td><td>3500-000-EL</td><td></td></tr><tr><td>DMEM Media</td><td>Wisent</td><td>319-005-CL</td><td></td></tr><tr><td>Fetal Bovine Serum (FBS)</td><td>Wisent</td><td>080-150</td><td></td></tr><tr><td>PBS</td><td>Wisent</td><td>311-010-CL</td><td></td></tr><tr><td>18 mm circular glass coverslips #1.5 thickness</td><td>Electron Microscopy Sciences</td><td>72290-08</td><td>Size and shape of coverslip is not critical, but 18 mm fit into the wells of a standard 12-well plate which simplifies cell culture</td></tr><tr><td>Staurosporine</td><td>Cayman Chemical</td><td>81590</td><td>Dissolve in DMSO at 1 mM (1,000x stock solution)</td></tr><tr><td>Annexin V-Alexa 488</td><td>ThermoFisher</td><td>R37174</td><td></td></tr><tr><td>EZ-Link NHS-Biotin</td><td>ThermoFisher</td><td>20217</td><td>Store in a dessicator. Do not prepare a stock solution.</td></tr><tr><td>DMSO</td><td>Sigma-Aldrich</td><td>D2650</td><td></td></tr><tr><td>CellTrace FarRed</td><td>ThermoFisher</td><td>C34572</td><td></td></tr><tr><td>CellTrace Orange</td><td>ThermoFisher</td><td>C34851</td><td></td></tr><tr><td>Hoescht 33342</td><td>ThermoFisher</td><td>62249</td><td></td></tr><tr><td>FITC-Streptavadin</td><td>ThermoFisher</td><td>SA1001</td><td></td></tr><tr><td>Lympholyte-poly cell sepration medium</td><td>Cedarlane Labs</td><td>CL5071</td><td></td></tr><tr><td>Recombinant Human M-CSF</td><td>Peprotech</td><td>200-04</td><td></td></tr><tr><td>Recombinant Human IL-4</td><td>Peprotech</td><td>300-25</td><td></td></tr><tr><td>J774.2 Macrophage Cell Line</td><td>Sigma-Aldrich</td><td>85011428-1VL</td><td></td></tr><tr><td>THP-1 Human Monocyte Cell Line</td><td>ATCC</td><td>TIB-202</td><td></td></tr><tr><td>Jurkat T Cell Line</td><td>ATCC</td><td>TIB-152</td><td></td></tr></tbody></table>

fixed cell efferocytosis assay: a method to study efferocytic uptake of apoptotic cells by macrophages using fluorescence microscopy

Source: Taruc, K., et al. <a href="https://appjove.unicartagenaproxy.elogim.com/v/58149">Quantification of Efferocytosis by Single-cell Fluorescence Microscopy.</a> J. Vis. Exp. (2018).
In this video, we demonstrate the efferocytosis assay to study the clearance of apoptotic cells using confocal microscopy. Efferocytosis is a multi-step process where apoptotic cells are engulfed by phagocytes and degraded within vesicles called efferosomes. This protocol provides a method to visualize internalized and non-internalized portions of individual apoptotic cells and quantify efferocytosis.

Fixed Cell Efferocytosis Assay: A Method to Study Efferocytic Uptake of Apoptotic Cells by Macrophages Using Fluorescence Microscopy

Source: Taruc, K., et al. Quantification of Efferocytosis by Single-cell Fluorescence Microscopy. J. Vis. Exp. (2018).
In this video, we demonstrate the ...

Cells undergoing apoptosis - programmed cell death - display eat-me signals on their cell surface, facilitating degradation by phagocytes - specialized immune cells. This process of clearance of apoptotic cells is called efferocytosis.
To perform the efferocytosis assay, first, take a suspension of dual-stained apoptotic cells. The surfaces of these cells are labeled with biotin, and the cytoplasm is labeled with a cell-tracking dye, tagging apoptotic cell-derived materials.
Add the cell suspension into a culture of adhered macrophage cells, which function as efferocytes. Centrifuge, forcing contact between macrophages and apoptotic cells, and incubate.
Efferocytic receptors on macrophages bind to phosphatidylserine - an eat-me signal - on the apoptotic cell membrane, facilitating its engulfment. Small fragments of the apoptotic cell are taken up inside a membrane-bound vesicle, called an efferosome.
This results in an efferocytosed fraction - part of the apoptotic cell inside the macrophage - and a non-efferocytosed fraction - the non-internalized part of the apoptotic cell.
Add fluorescently-labeled streptavidin, which binds to the exposed biotin molecules on the surface of the non-efferocytosed fraction, differentiating the non-internalized and internalized portions of the apoptotic cell.
Under a fluorescence microscope, the non-internalized apoptotic cell fraction shows streptavidin labeling, whereas efferosomes appear as discrete dots free of streptavidin.
To quantify efferocytosis, determine the number of discrete efferosomes, and measure the intensity of the efferocytosed and non-efferocytosed apoptotic cell fractions.

fixed-cell-efferocytosis-assay-method-to-study-efferocytic-uptake

Universidad de Cartagena UDEC

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569 Views. Fonte: Taruc, K., et al. Quantificazione dell'efferocitosi mediante microscopia a fluorescenza a cellula singola. J. Vis. Exp. (2018). In questo video, dimostriamo il test di efferocitosi per studiare la clearance delle cellule apoptotiche utilizzando la microscopia confocale. L'efferocitosi è un processo in più fasi in cui le cellule apoptotiche vengono inghiottite dai fagociti e degradate all'interno di vescicole chiamate efferosomi. Questo protocollo fornisce un metodo per visualizzare por...

Video: Saggio di efferocitosi cellulare fissa: un metodo per studiare l'assorbimento efferocitico delle cellule apoptotiche da parte dei macrofagi utilizzando la microscopia a fluorescenza - Concept

High Throughput Fluorometric Technique for Assessment of Macrophage Phagocytosis and Actin Polymerization

The goal of fluorometric analysis is to serve as an efficient, cost effective, high throughput method of analyzing phagocytosis and other cellular processes. This technique can be used on a variety of cell types, both adherent and non-adherent, to examine a variety of cellular properties. When studying phagocytosis, fluorometric technique utilizes phagocytic cell types such as macrophages, and fluorescently labeled opsonized particles whose fluorescence can be extinguished in the presence of trypan blue. Following plating of adherent macrophages in 96-well plates, fluorescent particles (green or red) are administered and cells are allowed to phagocytose for varied amounts of time. Following internalization of fluorescent particles, cells are washed with trypan blue, which facilitates extinction of fluorescent signal from bacteria which are not internalized, or are merely adhering to the cell surface. Following the trypan wash, cells are washed with PBS, fixed, and stained with DAPI (nuclear blue fluorescent label), which serves to label nuclei of cells. By a simple fluorometric quantification through plate reading of nuclear (blue) or particle (red/green) fluorescence we can examine the ratio of relative fluorescence units of green:blue and determine a phagocytic index indicative of amount of fluorescent bacteria internalized per cell. The duration of assay using a 96-well method and multichannel pipettes for washing, from end of phagocytosis to end of data acquisition, is less than 45 min. Flow cytometry could be used in a similar manner but the advantage of fluorometry is its high throughput, rapid method of assessment with minimal manipulation of samples and quick quantification of fluorescent intensity per cell. Similar strategies can be applied to non adherent cells, live labeled bacteria, actin polymerization, and essentially any process utilizing fluorescence. Therefore, fluorometry is a promising method for its low cost, high throughput capabilities in the study of cellular processes.

Here we present a protocol to quantify phagocytosis of fluorescent particles by adherent macrophage cell line using a fluorometric method. This method facilitates a high throughput quantification of particle internalization as well as the resulting actin polymerization.

Alta Tecnica Throughput fluorometrica per la valutazione dei macrofagi fagocitosi e polimerizzazione

The goal of fluorometric analysis is to serve as an efficient, cost effective, high throughput method of analyzing phagocytosis and other cellular ...

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Immunologia e infezioni

Experimental Analysis of Apoptotic Thymocyte Engulfment by Macrophages

Cell apoptosis is a natural process and plays a critical role in embryonic development, homeostatic regulation, immune tolerance induction, and resolution of inflammation. Accumulation of apoptotic debris in the body may trigger chronic inflammatory responses that lead to systemic autoimmune diseases over time. Impaired apoptotic cell clearance has been implicated in a variety of autoimmune diseases. Apoptotic clearance is a complex process rarely detected under physiological conditions. It involves abundant surface receptors and signaling molecules. Studying the process of apoptotic cell clearance provides insightful molecular mechanisms and subsequent biological responses, which may lead to the development of new therapeutics. Here, we describe protocols for the induction of apoptotic thymocytes, the preparation of peritoneal macrophages, and the analysis of apoptotic cell clearance by flow cytometry and microscopy. All cells will undergo apoptosis at a certain stage, and many residential and circulating cells can uptake apoptotic debris. Therefore, the protocol described here can be used in many applications to characterize apoptotic cell binding and ingestion by many other cell types.

Here, we present a protocol to prepare apoptotic thymocytes and peritoneal macrophages and analyze the efficiency of efferocytosis and the specific inhibitor-mediated blocking of apoptotic thymocytes engulfment. This protocol has a broad application in cell-mediated clearance of other particles including artificial beads and bacteria.

Analisi sperimentale di apoptotic thymocyte engulfment da macrofagi

Cell apoptosis is a natural process and plays a critical role in embryonic development, homeostatic regulation, immune tolerance induction, and resolution ...

In Vivo Assessment of Alveolar Macrophage Efferocytosis Following Ozone Exposure

Ozone (O3) is a criteria air pollutant that exacerbates and increases the incidence of chronic pulmonary diseases. O3 exposure is known to induce pulmonary inflammation, but little is known regarding how exposure alters processes important to the resolution of inflammation. Efferocytosis is a resolution process, whereby macrophages phagocytize apoptotic cells. The purpose of this protocol is to measure alveolar macrophage efferocytosis following O3-induced lung injury and inflammation. Several methods have been described for measuring efferocytosis; however, most require ex vivo manipulations. Described in detail here is a protocol to measure in vivo alveolar macrophage efferocytosis 24 h after O3 exposure, which avoids ex vivo manipulation of macrophages and serves as a simple technique that can be used to accurately represent perturbations in this resolution process. The protocol is a technically non-intensive and relatively inexpensive method that involves whole-body O3 inhalation followed by oropharyngeal aspiration of apoptotic cells (i.e., Jurkat T cells) while under general anesthesia. Alveolar macrophage efferocytosis is then measured by light microscopy evaluation of macrophages collected from bronchoalveolar (BAL) lavage. Efferocytosis is finally measured by calculating an efferocytic index. Collectively, the outlined methods quantify efferocytic activity in the lung in vivo while also serving to analyze the negative health effects of O3 or other inhaled insults.

This manuscript describes a protocol for determining whether exposure to ozone, a criteria air pollutant, impairs alveolar macrophage efferocytosis in vivo. This protocol utilizes commonly used reagents and techniques and can be adapted to multiple models of pulmonary injury to determine effects on alveolar macrophage efferocytosis.

Fixed Cell Efferocytosis Assay: A Method to Study Efferocytic Uptake of Apoptotic Cells by Macrophages Using Fluorescence Microscopy

Trascrizione

Fixed Cell Efferocytosis Assay: A Method to Study Efferocytic Uptake of Apoptotic Cells by Macrophages Using Fluorescence Microscopy