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This protocol outlines a method for quantifying the total biomass of Scleractinian coral samples which have been ground into a homogenous paste consisting of aragonite skeleton, coral host tissue, and endosymbiotic Symbiodiniaceae cells. There are four parts to quantifying total biomass: 1) grind coral fragments into a homogenous paste, 2) partition the biomass subsample, 3) quantify the ash-free dry weight [AFDW], and 4) standardize AFDW to the colony surface area. This method has been reported in several publications by Grottoli's team (e.g., Rodrigues & Grottoli 2007). This protocol was written by Rowan McLachlan (03-19-20) and was reviewed by all co-authors. dx.doi.org/10.17504/protocols.io.bdyai7se 

This protocol outlines a method for quantifying the density of Symbiodiniaceae cells in Scleractinian coral samples which have been previously ground into a homogenous paste consisting of aragonite skeleton, coral host tissue and endosymbiotic Symbiodiniaceae cells. There are four parts to quantifying Symbiodiniaceae cell density from ground corals: 1) grind and sub-sample the coral and store at -80 °C until ready to extract, 2) separate Symbiodiniaceae cells from the coral skeleton, 3) image Symbiodiniaceae fluorescence using Countess™ II FL Automated Cell Counter, and 4) quantify cells using the software ImageJ. Note: a CY5 EVOS™ light cube is required for this method. For instructions on installing the CY5 EVOS™ light cube to your Countess™ II FL Cell Counter, see page 40 of the Countess™ II FL Cell Counter user manual. This method was originally developed by Rowan McLachlan in February 2020. Claire Juracka assisted Rowan McLachlan by conducting tests to compare this method to the traditional method using a hemocytometer and microscope. The traditional cell counting method has been reported in several publications by Grottoli's team (e.g., Rodrigues & Grottoli 2007). This protocol was written by Rowan McLachlan with the guidance of Dr. Andréa Grottoli at The Ohio State University. dx.doi.org/10.17504/protocols.io.bdc5i2y6 

This method is adapted and updated from methods originally published in Grottoli et al. (2004) and is based on the original methods of Folch & Stanley (1957), and Bligh & Dyer (1959). There are five parts to extracting lipids from ground corals: 1) grind and sub-sample the coral and store at -80 °C until ready to extract, 2) freeze-dry the sample, 3) extract the lipids from the freeze-dried samples, 4) standardize the lipid concentration to ash-free dry weight (AFDW), and 5) resuspend the extracted lipid for long-term storage and possible later analysis of lipid classes or isotopes. The lipid extraction procedure must be conducted in a fume hood with the sash as low as possible with the researcher wearing protective eyewear, gloves, and lab coat at all times. Important considerations regarding lipid analysis were gained from reading Chapter 1.3 “Lipid extraction, storage, and sample handling” from the textbook Lipid Analysis by Christie (2003). This method was originally developed by Andréa Grottoli and refined by Rowan McLachlan (06-11-18) with the guidance of Dr. Agus Muñoz-Garcia at The Ohio State University. This protocol was written by Rowan McLachlan (03-12-2020). dx.doi.org/10.17504/protocols.io.bc4qiyvw 

This method for extracting protein from ground coral samples is based on the Bradford assay for the colorimetric detection and quantification of total protein (Bradford, 1976) and is compared to a known standard dilution of bovine serum albumin (BSA). Pierce Inc. and Bio-Rad have developed the reagents and standards necessary for completing the extraction. There are five parts to quantifying total soluble protein in ground corals: 1) grind and sub-sample the coral and store at -80 °C until ready to extract, 2) solubilize protein via cell disruption [detergent lysis and freeze-thaw lysis], 3) separate the dissolved protein from tissue and skeletal particles, 4) quantify the protein concentration via Bradford microassay procedure, and 5) standardize the protein concentration to ashfree dry weight (AFDW). This method was originally developed by Rowan McLachlan with the assistance of Jamie Price and Kerri Dobson and with the guidance of Dr. Noah Weisleder and Andréa Grottoli at The Ohio State University. This protocol was written by Rowan McLachlan and reviewed by all co-authors. dx.doi.org/10.17504/protocols.io.bdc8i2zw 

Coral bleaching is the single largest global threat to coral reefs worldwide. Integrating the diverse body of work on coral bleaching is critical to understanding and combating this global problem. Yet investigating the drivers, patterns, and processes of coral bleaching poses a major challenge. A recent review of published experiments revealed a wide range of experimental variables used across studies. Such a wide range of approaches enhances discovery, but without full transparency in the experimental and analytical methods used, can also make comparisons among studies challenging. To increase comparability but not stifle innovation, we propose a common framework for coral bleaching experiments that includes consideration of coral provenance, experimental conditions, and husbandry. For example, reporting the number of genets used, collection site conditions, the experimental temperature offset(s) from the maximum monthly mean (MMM) of the collection site, experimental light conditions, flow, and the feeding regime will greatly facilitate comparability across studies. Similarly, quantifying common response variables of endosymbiont (Symbiodiniaceae) and holobiont phenotypes (i.e., color, chlorophyll, endosymbiont cell density, mortality, and skeletal growth) could further facilitate cross‐study comparisons. While no single bleaching experiment can provide the data necessary to determine global coral responses of all corals to current and future ocean warming, linking studies through a common framework as outlined here, would help increase comparability among experiments, facilitate synthetic insights into the causes and underlying mechanisms of coral bleaching, and reveal unique bleaching responses among genets, species, and regions. Such a collaborative framework that fosters transparency in methods used would strengthen comparisons among studies that can help inform coral reef management and facilitate conservation strategies to mitigate coral bleaching worldwide.