Name: cycloheximide chase analysis of protein degradation in saccharomyces cerevisiae
Uploaded: 2016-04-18T15:00:00.000+00:00
Duration: 9 min 5 s
Description: Watch this Scientific Journal Video about Cycloheximide Chase Analysis of Protein Degradation in Saccharomyces cerevisiae at JoVE.com

The authors thank current and former members of the Rubenstein lab for providing a supportive and enthusiastic research environment. The authors thank Mark Hochstrasser (Yale University) for sharing reagents and expertise. E.M.R. thanks Stefan Kreft (University of Konstanz) and Jennifer Bruns (University of Pittsburgh) for sharing invaluable expertise in kinetic analysis of proteins. This work was supported by a National Institutes of Health grant (R15 GM111713) to E.M.R., a Ball State University ASPiRE research award to E.M.R, a research award from the Ball State University chapter of Sigma Xi to S.M.E., and funds from the Ball State University Provost's Office and Department of Biology.

1. Growth and Harvest of Yeast Cells
<ol>
	<li>If not analyzing degradation kinetics of an endogenous yeast protein, transform desired yeast strain(s) with a plasmid encoding the protein of interest. Reliable methods for yeast transformation have been previously described 37.</li>
	<li>Inoculate yeast in 5 ml of appropriate medium (e.g., selective synthetic defined (SD) medium for plasmid maintenance of transformed cells or non-selective yeast extract-peptone-dextrose (YPD) medium for non-transformed cells). Incubate overnight at 30 &#176;C, rotating. 
	NOTE: 30 &#176;C is the optimal growth temperature for typical wild-type laboratory yeast strains 38. However, because some mutant yeast strains do not grow optimally at 30 &#176;C and some proteins undergo temperature-dependent degradation, the temperatures used for yeast cell growth and cycloheximide chase should be empirically determined 39.</li>
	<li>Measure the optical density at 600 nm (OD600) of each overnight culture. 
	NOTE: Cells may be in logarithmic or stationary growth phase but should have minimally reached a density that will allow dilution to an OD600 = 0.2 in 15 ml of fresh medium.</li>
	<li>Dilute the overnight cultures to an OD600 value of 0.2 in 15 ml of fresh medium.</li>
	<li>Incubate yeast at 30 &#176;C, shaking until the cells reach mid-logarithmic growth phase (i.e., an OD600 between 0.8 and 1.2).</li>
	<li>During yeast cell growth, perform the following in preparation for the cycloheximide chase procedure:
	<ol>
		<li>Set a heat block that can accommodate 15 ml conical tubes to 30 &#176;C for incubation of cells in the presence of cycloheximide. Add water to the wells of the heat block to allow efficient heat distribution to cultures. Add water to each well such that a 15 ml conical tube will cause the water level to rise to, but not overflow, the lip of the well.</li>
		<li>Set a second heat block that can accommodate 1.5 ml microcentrifuge tubes to 95 &#176;C for protein denaturation following cell lysis.</li>
		<li>Pre-warm fresh growth medium (1.1 ml per time point per culture to be assayed) to 30 &#176;C.</li>
		<li>Add 50 &#181;l 20x Stop Mix to pre-labeled microcentrifuge tubes (one tube per time point per culture to be assayed). Place tubes on ice. 
		CAUTION: Sodium azide, an ingredient in 20x Stop Mix, is toxic via oral ingestion or dermal contact. Follow manufacturer recommendations when preparing, storing, and handling sodium azide. In the event of accidental exposure, consult material safety data sheet provided by manufacturer.</li>
	</ol>
	</li>
	<li>When cells have reached mid-logarithmic growth, collect 2.5 OD600 units of each culture per time point to be assayed (e.g., 7.5 OD600 units to analyze protein abundance at three time points). Centrifuge collected cells in 15 ml conical tubes at 3,000 x g at room temperature for 2 min. 
	NOTE: One OD600 unit is equal to the amount of yeast present in 1 ml culture at an OD600 of 1.0. The volume of culture (in ml) required to harvest X OD600 units (V) may be determined by using the following equation: V = X OD600 units/Measured OD600. For example, to harvest 7.5 OD600 units of yeast cell culture at an OD600 of 1.0, collect 7.5 OD600 units/1.0 = 7.5 ml yeast culture.</li>
	<li>Resuspend each cell pellet in 1 ml of 30 &#176;C (pre-warmed) fresh growth medium per 2.5 OD600 units of cells (e.g., 3 ml for 7.5 OD600 units).</li>
</ol>
2. Cycloheximide Chase
<ol>
	<li>Equilibrate yeast cell suspensions by incubation for 5 min in the 30 &#176;C heat block.</li>
	<li>Prepare a timer to count up from 0:00.</li>
	<li>To begin the cycloheximide chase, press &#34;Start&#34; on the timer. Swiftly, but carefully, perform the following steps:
	<ol>
		<li>Add cycloheximide to a final concentration of 250 &#181;g/ml to the first yeast cell suspension (e.g., add 37.5 &#181;l of 20 mg/ml cycloheximide stock to 3 ml of cell suspension), and vortex briefly to mix. 
		CAUTION: Cycloheximide is a dermal irritant and is toxic via oral ingestion. Follow manufacturer recommendations when preparing, storing, and handling cycloheximide. In the event of accidental exposure, consult material safety data sheet provided by manufacturer.</li>
		<li>Immediately after adding cycloheximide and vortexing, transfer 950 &#181;l (~2.4 OD600 units) of the yeast cell suspension with added cycloheximide to a pre-labeled microcentrifuge tube containing 50 &#181;l ice-cold 20x stop mix. Vortex the microcentrifuge tube, and place on ice until all samples have been collected.</li>
		<li>Return the yeast cell suspension to 30 &#176;C.</li>
	</ol>
	</li>
	<li>Repeat steps 2.3.1 through 2.3.3 for each of the remaining yeast cell suspensions at regular time intervals (e.g., every 30 sec, such that cycloheximide is added to Sample #1 at 0:00, Sample #2 at 0:30, Sample #3 at 1:00, etc.).</li>
	<li>At each subsequent time point, vortex yeast cell suspensions and transfer 950 &#956;l to labeled microcentrifuge tubes containing 50 &#956;l pre-chilled 20x Stop Mix. Vortex and place collected cells on ice. Return 15 ml conical tubes to 30 &#176;C heat block.
	<ol>
		<li>For example, for collection of cells 30 min after cycloheximide addition (assuming 30-sec intervals between cycloheximide addition to yeast cell suspensions at the beginning of the time course), vortex and remove 950 &#956;l of cell suspension from Sample #1 at 30:00. Repeat for Sample #2 at 30:30, and so on. 
		NOTE: To prevent settling of yeast, vortex cell suspensions in 15 ml conical tubes approximately every 5 min throughout the course of the chase. Alternatively, yeast cell suspensions may be maintained in a continuously agitating water bath for the duration of the cycloheximide chase experiment.</li>
	</ol>
	</li>
	<li>When all samples have been collected, pellet collected cells by centrifugation at 6,500 x g at room temperature for 30 sec. Remove the supernatant by pipetting or aspiration. Cells are now ready for alkaline lysis. Alternatively, snap-freeze pelleted cells in liquid nitrogen and store at -80 &#176;C.</li>
</ol>
3. Post-alkaline Protein Extraction (Modified from 16,40)
<ol>
	<li>Add 100 &#181;l of distilled water to each cell pellet. Resuspend by pipetting up and down or vortexing.</li>
	<li>Add 100 &#181;l&#160;of 0.2 M NaOH to each sample. Mix by pipetting up and down or vortexing.</li>
	<li>Incubate suspended cells at room temperature for 5 min. At this stage, yeast cells have not been lysed, and proteins have not been released 40.</li>
	<li>Pellet cells by centrifugation at 18,000 x g at room temperature for 30 sec. Remove supernatant by pipetting or aspiration.</li>
	<li>To lyse cells, add 100 &#181;l of Laemmli sample buffer to each cell pellet. Resuspend by pipetting up and down or vortexing. 
	NOTE: Sequential incubation of cells with NaOH and Laemmli sample buffer releases proteins in a form compatible with sodium dodecyl sulfate-polyacrylamide gel electrophoresis (SDS-PAGE) using a Tris-glycine running buffer system.</li>
	<li>Incubate at 95 &#176;C for 5 min to fully denature proteins. 
	NOTE: Incubation at 95 &#176;C may not be suitable for analysis of proteins that are prone to aggregation (e.g., proteins with several transmembrane segments). These proteins may become insoluble when incubated at elevated temperatures 41. Thus, for the analysis of such proteins, lysates should be incubated at lower temperatures (e.g., 37 &#176;C - 70 &#176;C) for 10 - 30 min, as empirically determined.</li>
	<li>Centrifuge lysates at 18,000 x g at room temperature for 1 min to pellet insoluble material. The supernatant (solubilized extracted protein) is ready for separation by SDS-PAGE and subsequent western blot analysis. Alternatively, store lysates at -20 &#176;C.</li>
</ol>
4. Representative SDS-PAGE and Western Blotting Procedure (Adapted from 16)
<ol>
	<li>Load protein molecular weight standards and empirically determined volume of lysates onto an SDS-PAGE gel. 
	NOTE: Choose the percentage of acrylamide and bis-acrylamide in the SDS-PAGE gel based on the molecular weight of the protein of interest. In general, lower percentage gels are better suited for resolving higher molecular weight proteins.</li>
	<li>Run gel at 200 V until the dye front has reached the bottom edge of the gel.</li>
	<li>Transfer proteins from the gel to polyvinylidene fluoride (PVDF) membrane by wet transfer at 20 V for 60 - 90 min at 4 &#176;C.</li>
	<li>Block membrane by incubating in Tris-Buffered Saline (TBS) containing 5% skim milk, rocking, at room temperature for 1 hr or at 4 &#176;C overnight. 
	NOTE: To prevent microbial growth in the presence of a membrane incubated overnight, it is recommended to include sodium azide in the blocking solution at a final concentration of 0.02%.</li>
	<li>Incubate membrane with primary antibody specific for protein of interest in TBS with 0.1% Tween-20 (TBS/T) and 1% skim milk, rocking, at room temperature for 1 hr.</li>
	<li>Wash membrane at room temperature 3 x 5 min with TBS/T, rocking.</li>
	<li>Incubate membrane with appropriate fluorophore-conjugated secondary antibody in TBS/T with 1% skim milk at room temperature for 1 hr, rocking. 
	NOTE: Fluorophores are light-sensitive. Therefore, dilutions of antibodies conjugated to fluorophores should be prepared in the dark, and incubation of membranes in the presence of antibodies conjugated to fluorophores and subsequent wash steps should occur in lightproof (e.g., foil-wrapped) containers.</li>
	<li>Wash membrane at room temperature 3 x 5 min with TBS/T, rocking.</li>
	<li>Image membrane using LI-COR Odyssey CLx and Image Studio software (or comparable imaging equipment and software), following manufacturer recommendations.</li>
	<li>After acquiring membrane image, incubate the membrane with a primary antibody specific for a loading control protein in TBS/T with 1% skim milk at room temperature for 1 hr, rocking.</li>
	<li>Wash membrane at room temperature 3 x 5 min with TBS/T, rocking.</li>
	<li>Incubate membrane with appropriate fluorophore-conjugated secondary antibody in TBS/T with 1% skim milk at room temperature for 1 hr, rocking.</li>
	<li>Wash membrane at room temperature 3 x 5 min with TBS/T, rocking.</li>
	<li>Image membrane as in step 4.9.</li>
</ol>

The authors have nothing to disclose.

In this paper, a method for analyzing protein degradation kinetics is presented. This technique can be readily applied to a range of proteins degraded by a variety of mechanisms. It is important to note that cycloheximide chase experiments report on degradation kinetics of the steady state pool of a given protein. Other techniques may be used to analyze the degradation kinetics of specific populations of proteins. For example, the degradative fate of nascent polypeptides can be tracked by pulse chase analysis 55. In such experiments, nascent proteins are briefly pulse-labeled (e.g., with radioactive amino acids). Changes in the abundance of the labeled nascent proteins (which may or may not mirror changes in steady state protein abundance) may be tracked over time.
Cycloheximide chase is suitable for analyzing protein stability over a relatively short time course (i.e., up to two hours). Over longer time courses (i.e., two hours to days), cycloheximide, a global inhibitor of translation, is toxic to cells, likely due to depletion of ubiquitin 56. Further, analyses of protein stability over longer time courses are more likely to be compromised by indirect effects of globally impaired protein synthesis on the degradation of the protein of interest (e.g., degradation of a short-lived protein involved in the degradation of the protein of interest). Other techniques, such as pulse chase metabolic labeling experiments, are therefore better suited for studying the degradation of long-lived proteins and may be performed to corroborate results obtained in cycloheximide chase experiments.
The timing of addition of cycloheximide and collection of cells is an important consideration in this procedure. Precision is especially important in the analysis of very short-lived proteins, as small deviations in the time elapsed from cycloheximide addition to cell harvest can have a substantial impact on apparent degradation kinetics. Further, without a clear plan for executing these time-sensitive steps, an experiment may rapidly devolve into chaos and frustration. For this reason, it is recommended to add cycloheximide to cultures at planned, regular intervals. 30-sec intervals are suggested in this protocol, but the timing may be adjusted to match the comfort level and dexterity of the investigator. Novice investigators may find it useful to write a schedule of sample collection times prior to initiating the experiment and to cross off each scheduled collection as it occurs.
In Steps 1.7 and 1.8 of the protocol described here, yeast cell cultures are concentrated in reduced volumes of growth medium for ease of manipulation during the subsequent cycloheximide chase procedure. However, centrifugation of yeast cells rapidly induces certain cellular stress responses (e.g., signaling pathways that are activated by glucose deprivation) 57,58. Investigators are therefore cautioned against extended periods of centrifugation. When analyzing the stability of proteins that may be sensitive to centrifugation, investigators may wish to add cycloheximide directly to mid-log phase cultures without prior centrifugation. In such cases, cycloheximide should be added to the same final concentration (250 &#956;g/ml), and yeast cell samples may be harvested by methodologies that do not require an initial centrifugation step (e.g., rapid filtration) 57. Further, in Steps 2.3 - 2.5, samples collected at each time point are transferred to a solution containing sodium azide and placed on ice. These conditions inhibit continued protein degradation for the duration of the chase. It should be noted that azide reduces the cellular concentration of ATP 59, thereby specifically inhibiting the activity of ATP-dependent proteases. While reduced temperature should also reduce the rate at which non-ATP-dependent proteolytic processes function, investigators studying proteins degraded by such mechanisms may alternatively choose to snap-freeze cell pellets in liquid nitrogen as each sample is harvested.
A sample protocol for cell lysis and a representative protocol for western blotting included in this manuscript have been adapted from previous reports 16,40. In the post-alkaline lysis method described here, NaOH pretreatment enhances extraction of yeast proteins upon subsequent addition of Laemmli sample buffer. The mechanism by which this enhancement occurs is poorly characterized 40. However, polysaccharides such as those found in yeast cell walls are solubilized in alkali conditions 60. It is therefore tempting to speculate that incubation in the presence of NaOH partially or completely spheroplasts yeast cells (i.e., removes cell wall components), rendering them more sensitive to the SDS detergent present in the Laemmli sample buffer. Because proteins are released under highly denaturing conditions, protease inhibitors need not be included in the Laemmli sample buffer. The specific method of cell lysis may be modified as appropriate for a given experiment. For instance, the post-alkaline lysis method may not be suitable for low-abundance proteins or proteins that are poorly detected by western blot. In such cases, methods that include a trichloroacetic acid precipitation step to concentrate protein samples may be most appropriate 61. Moreover, several important considerations regarding antibody selection, loading control choice, and alternative means of detection (e.g., chemiluminescent western blotting using film or digital imaging systems) have been recently discussed 16. Quantitation of protein abundance following cycloheximide treatment may be performed. Many imaging systems are sold with software packages that facilitate this analysis.
Cycloheximide chase may be implemented to analyze the degradation of a variety of yeast proteins and may be adapted to study protein stability in other eukaryotic cells. As described in this protocol, cycloheximide treatment is followed by cell lysis and detection of protein abundance by western blot analysis. Depending on the application, however, protein abundance following cycloheximide treatment may be assessed by a range of techniques, as appropriate for research objectives. For example, if protein size is not a relevant factor for analysis, cell lysates may be subjected to dot blot or enzyme-linked immunosorbent assay (ELISA) analysis, which report on protein abundance, but not apparent molecular weight 62. For proteins on the cell surface (or internal fluorescently tagged internal proteins), flow cytometry may be used to quantify protein abundance of samples at different times after cycloheximide addition 51. Fluorescence microscopy following cycloheximide treatment would provide information on both protein abundance and localization 18. The range of substrates, organisms, and downstream applications amenable to cycloheximide chase makes the technique a highly versatile and informative means of studying protein degradation.

Proteins perform crucial functions in virtually every cellular process. Many physiological processes require the presence of a specific protein (or proteins) for a defined period of time or under particular circumstances. Organisms therefore monitor and regulate protein abundance to meet cellular needs 1. For example, cyclins (proteins that control cell division) are present at specific phases of the cell cycle, and the loss of regulated cyclin levels has been associated with malignant tumor formation 2. In addition to regulating protein levels to meet cellular needs, cells employ degradative quality control mechanisms to eliminate misfolded, unassembled, or otherwise aberrant protein molecules 3. Control of protein abundance involves regulation of both macromolecular synthesis (transcription and translation) and degradation (RNA decay and proteolysis). Impaired or excessive protein degradation contributes to multiple pathologies, including cancer, cystic fibrosis, neurodegenerative conditions, and cardiovascular disorders 4-8. Proteolytic mechanisms therefore represent promising therapeutic targets for a range of illnesses 9-12.
Analysis of proteins at a single time point (e.g., by western blot 13, flow cytometry 14, or fluorescence microscopy 15) provides a snapshot of steady state protein abundance without revealing the relative contributions of synthesis or degradation. Similarly, growth-based reporter assays reflect steady state protein levels over an extended time period without discriminating between the influences of synthesis and degradation 15-20. It is possible to infer the contribution of degradative processes to steady state protein levels by comparing abundance before and after inhibiting specific components of the degradative mechanism (e.g., by pharmacologically inactivating the proteasome 21 or knocking out a gene hypothesized to be required for degradation 13). A change in steady state protein levels after inhibiting degradative pathways provides strong evidence for the contribution of proteolysis to the control of protein abundance 13. However, such an analysis still does not provide information regarding the kinetics of protein turnover. Cycloheximide chase followed by western blotting overcomes these weaknesses by allowing researchers to visualize protein degradation over time 22-24. Further, because protein detection following cycloheximide chase is typically performed by western blotting, radioactive isotopes and lengthy immunoprecipitation steps are not required for cycloheximide chase, unlike many commonly used pulse chase techniques, which are also performed to visualize protein degradation25.
Cycloheximide was first identified as a compound with anti-fungal properties produced by the gram-positive bacterium Streptomyces griseus 26,27. It is a cell-permeable molecule that specifically inhibits eukaryotic cytosolic (but not organellar) translation by impairing ribosomal translocation 28-31. In a cycloheximide chase experiment, cycloheximide is added to cells, and aliquots of cells are collected immediately and at specific time points following addition of the compound 22. Cells are lysed, and protein abundance at each time point is analyzed, typically by western blot. Decreases in protein abundance following the addition of cycloheximide can be confidently attributed to protein degradation. An unstable protein will decrease in abundance over time, while a relatively stable protein will exhibit little change in abundance.
Mechanisms of selective protein degradation have been highly conserved throughout Eukarya. Much of what is known about protein degradation was first learned in the model unicellular eukaryote, Saccharomyces cerevisiae (budding yeast) 25,32-36. Studies with yeast are likely to continue providing novel and important insights into protein degradation. A method for cycloheximide chase in yeast cells followed by western blot analysis of protein abundance is presented here.

<table><tbody><tr><td>Desired yeast strains, plasmids, standard medium and buffer components</td><td></td><td></td><td></td></tr><tr><td>Disposable borosilicate glass tubes</td><td>Fisher Scientific</td><td>14-961-32</td><td>Available from a variety of manufacturers</td></tr><tr><td>Temperature-regulated incubator (&lt;em&gt;e.g.&lt;/em&gt; Heratherm Incubator Model IMH180)</td><td>Dot Scientific</td><td>51028068</td><td>Available from a variety of manufacturers</td></tr><tr><td>New Brunswick Interchangeable Drum for 18 mm tubes (tube roller)</td><td>New Brunswick</td><td>M1053-0450</td><td>A tube roller is recommended to maintain overnight&amp;nbsp; starter cultures of yeast cells in suspension. Alternatively, if a tube roller is unavailable, a platform shaker in a temperature-controlled incubator may be used for overnight starter cultures. A platform shaker or tube roller may be used to maintain larger cultures in suspension.</td></tr><tr><td>New Brunswick TC-7 Roller Drum 120 V 50/60 H</td><td>New Brunswick</td><td>M1053-4004</td><td>For use with tube roller</td></tr><tr><td>SmartSpec Plus Spectrophotometer</td><td>Bio-Rad</td><td>170-2525</td><td>Available from a variety of manufacturers</td></tr><tr><td>Centrifuge 5430</td><td>Eppendorf</td><td>5427 000.216&amp;nbsp;</td><td>Rotor that is sold with unit holds 1.5 and 2.0 ml microcentrifuge tubes. Rotor may be swapped for one that holds 15 and 50 ml conical tubes</td></tr><tr><td>Fixed-Angle Rotor F-35-6-30 with Lid and Adapters for Centrifuge Model 5430/R, 15/50 ml Conical Tubes, 6-Place</td><td>Eppendorf</td><td>F-35-6-30</td><td></td></tr><tr><td>15-ml screen printed screw cap tube 17 x 20 mm conical, polypropylene</td><td>Sarstedt</td><td>62.554.205</td><td>Available from a variety of manufacturers</td></tr><tr><td>1.5-ml flex-tube, PCR clean, natural microcentrifuge tubes</td><td>Eppendorf</td><td>22364120</td><td>Available from a variety of manufacturers</td></tr><tr><td>Analog Dri-Bath Heaters</td><td>Fisher Scientific</td><td>1172011AQ</td><td>It is recomended that two heaters are available (one for incubating cells during cycloheximide treatment and one for boiling lysates to denature proteins). Alternatively, 30 &amp;deg;C water bath may be used for incubation of cells in the presence of cycloheximide. Boiling water bath with hot plate may altertnatively be used to denature proteins.</td></tr><tr><td>Heating block for 12 x 15 ml conical tubes</td><td>Fisher Scientific</td><td>11-473-70</td><td>For use with Dri-Bath Heater during incubation of cells in the presence of cycloheximide.</td></tr><tr><td>Heating block for 20 x 1.5 ml conical tubes</td><td>Fisher Scientific</td><td>11-718-9Q</td><td>For use with Dri-Bath Heater to boil lysates for protein denaturation.</td></tr><tr><td>SDS-PAGE running and transfer apparatuses, power supplies, and imaging equipment or darkrooms for SDS-PAGE and transfer to membrane</td><td></td><td></td><td>Will vary by lab and application</td></tr><tr><td>Western blot imaging system (&lt;em&gt;e.g.&lt;/em&gt; Li-Cor Odyssey CLx scanner and Image Studio Software)</td><td>Li-Cor</td><td>9140-01</td><td>Will vary by lab and application</td></tr><tr><td>EMD Millipore Immobilon PVDF Transfer Membranes</td><td>Fisher Scientific</td><td>IPFL00010</td><td>Will vary by lab and application</td></tr><tr><td>Primary antibodies (&lt;em&gt;e.g.&lt;/em&gt; Phosphoglycerate Kinase (Pgk1) Monoclonal antibody, mouse (clone 22C5D8))</td><td>Life Technologies</td><td>459250</td><td>Will vary by lab and application</td></tr><tr><td>Secondary antibodies (&lt;em&gt;e.g.&lt;/em&gt; Alexa-Fluor 680 Rabbit Anti-Mouse IgG (H + L))</td><td>Life Technologies</td><td>A-21065</td><td>Will vary by lab and application</td></tr></tbody></table>

cycloheximide chase analysis of protein degradation in saccharomyces cerevisiae

Regulation of protein abundance is crucial to virtually every cellular process. Protein abundance reflects the integration of the rates of protein synthesis and protein degradation. Many assays reporting on protein abundance (e.g., single-time point western blotting, flow cytometry, fluorescence microscopy, or growth-based reporter assays) do not allow discrimination of the relative effects of translation and proteolysis on protein levels. This article describes the use of cycloheximide chase followed by western blotting to specifically analyze protein degradation in the model unicellular eukaryote, Saccharomyces cerevisiae (budding yeast). In this procedure, yeast cells are incubated in the presence of the translational inhibitor cycloheximide. Aliquots of cells are collected immediately after and at specific time points following addition of cycloheximide. Cells are lysed, and the lysates are separated by polyacrylamide gel electrophoresis for western blot analysis of protein abundance at each time point. The cycloheximide chase procedure permits visualization of the degradation kinetics of the steady state population of a variety of cellular proteins. The procedure may be used to investigate the genetic requirements for and environmental influences on protein degradation.

To illustrate cycloheximide chase methodology, the stability of Deg1-Sec62 (Figure 1), a model yeast endoplasmic reticulum (ER)-associated degradation (ERAD) substrate, was analyzed 42-44. In ERAD, quality control ubiquitin ligase enzymes covalently attach chains of the small protein ubiquitin to aberrant proteins localized to the ER membrane. Such polyubiquitylated proteins are subsequently removed from the ER and degraded by the proteasome, a large, cytosolic protease 45. The Deg1-Sec62 protein is targeted for degradation after it persistently and aberrantly engages the translocon, a channel that facilitates protein translocation into the ER lumen or membrane 43. Similarly, mammalian apolipoprotein B, a protein component of low-density lipoproteins, persistently engages the ER translocon and subsequently undergoes degradation by a related mechanism when its lipid binding partners are absent 46-48. Thus, analyses of Deg1-Sec62 degradation in yeast cells may yield insight into the degradation of proteins that persistently or aberrantly engage the translocon, provisionally termed ERAD-T (for translocon-associated) substrates 43.
Previous studies have indicated that the ER-resident ubiquitin ligase Hrd1 functions with the ubiquitin-conjugating enzyme Ubc7 to catalyze degradation of Deg1-Sec62 16,42-44. The transmembrane protein Cue1 anchors Ubc7 to the ER membrane and activates the enzyme 49-51. However, a requirement for Cue1 in the degradation of Deg1-Sec62 has not been directly investigated. To test the hypothesis that Cue1, like Hrd1 and Ubc7, is required for efficient degradation of Deg1-Sec62, wild-type and mutant yeast cells expressing Deg1-Sec62 were subjected to cycloheximide chase and western blot analysis (Figure 2A). The Deg1-Sec62 protein migrates on SDS-PAGE as multiple species. This is consistent with earlier studies indicating extensive post-translational modification of the protein 43,44,52. In wild-type yeast cells, Deg1-Sec62 was readily degraded. As previously observed, loss of either Hrd1 or Ubc7 substantially stabilized the Deg1-Sec62 protein 42-44. As predicted, Deg1-Sec62 was stabilized in the absence of Cue1 (to a similar extent as in the absence of Ubc7), confirming a role for the Ubc7-interacting protein in ERAD-T.
The proportion of Deg1-Sec62 protein remaining at each time point was quantified and is plotted in Figure 2B. We note that the apparent rate of disappearance of Deg1-Sec62 in wild-type cells may be an underestimation of the rate of degradation of nascent Deg1-Sec62 (i.e., the protein's half-life, which can be most directly determined by pulse chase analysis 43). Because wild-type yeast actively degrade the Deg1-Sec62 protein prior to cycloheximide addition, steady state abundance of Deg1-Sec62 is substantially reduced in these cells (compared to cells in which degradation is impaired). This can be appreciated by comparing the abundance of Deg1-Sec62 at the initial time points for each strain in Figure 2A. Further, any degradation-resistant subpopulation of the substrate protein (e.g., if the protein accumulates in intracellular pools from which degradation is prevented) might appear relatively stable in wild-type cells over the time course of the experiment.
<img alt="Protein degradation diagram; endoplasmic reticulum-associated degradation process; ER membrane." src="/files/ftp_upload/53975/53975fig1.jpg" data-altupdatedat="1747911167000" data-alt="Figure 1"> 
Figure 1. Model for Degradation of Deg1-Sec62 following Aberrant Engagement of Translocon. (A) Schematic depiction of Deg1-Sec62. Deg1-Sec62 consists of the following elements, in sequence: Deg1 (the amino-terminal 67 amino acids from the yeast transcriptional repressor MATα2), a Flag (F) epitope, the 2-transmembrane protein Sec62, and two copies of the Staphylococcus aureus Protein A (PrA). (B) Following normal co-translational insertion of its two transmembrane segments into the endoplasmic reticulum (ER) membrane, persistent association of Deg1-Sec62 with the translocon triggers abnormal, Deg1-dependent, post-translational translocon engagement. A portion of the cytosolic amino terminus aberrantly enters-and likely remains within-the translocon. (C) Following translocon engagement, the Hrd1 ubiquitin ligase ubiquitylates Deg1-Sec62. Hrd1 is assisted by the ubiquitin-conjugating enzyme Ubc7, which is anchored in the ER membrane by Cue1. Ub, ubiquitin protein monomers. (D) Ubiquitylated Deg1-Sec62 is extracted from the ER membrane and degraded by the proteasome, relieving translocon obstruction. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/53975/53975fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Western blot and line graph; protein degradation over time under gene deletion conditions." src="/files/ftp_upload/53975/53975fig2.jpg" data-altupdatedat="1747911167000" data-alt="Figure 2"> 
Figure 2. Cycloheximide Chase followed by Western Blotting Indicates that Cue1 is Required for Efficient Deg1-Sec62 Degradation. (A) Yeast cells of the indicated genotypes were transformed with a yeast centromeric plasmid encoding Deg1-Sec62 (pRS416-PMET25-Deg1-Flag-Sec62-2xProtA; AmpR/URA343) and subjected to cycloheximide chase analysis. Proteins from each time point (equivalent to 0.125 OD600 units) were separated on an 8% SDS-PAGE gel and detected by western blotting with rabbit anti-mouse secondary antibodies, which directly bind the C-terminal Protein A epitopes of the Deg1-Sec62 fusion protein. As a loading control, the membrane was subsequently incubated with antibodies specific to Pgk1. This experiment has been replicated three times; representative results are pictured. (B) Quantification of data in (A) was performed using imaging software (see Table of Materials). The total fluorescence intensity of an area encompassing the Deg1-Sec62 protein was determined for each sample. Background fluorescence intensity for each sample was extrapolated from the average fluorescence intensity of pixels near the Deg1-Sec62 protein. This extrapolated background fluorescence intensity was subtracted from the total fluorescence intensity to yield adjusted fluorescence intensity for each sample. Similar quantifications for total, background, and adjusted fluorescence intensities were performed for Pgk1, a loading control protein whose abundance does not vary in the conditions assayed. To compare the abundance of Deg1-Sec62 protein among samples, a ratio of the adjusted signal intensities of Deg1-Sec62 to Pgk1 was determined for each sample. The Deg1-Sec62/Pgk1 ratio was defined as 100% for the first time point (i.e., immediately after cycloheximide addition) for each strain under analysis. The amount of Deg1-Sec62 remaining at subsequent time points (i.e., the Deg1-Sec62/Pgk1 ratios) was calculated as a percentage of the Deg1-Sec62/Pgk1 ratio at the first time point. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/53975/53975fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
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			<td rowspan="3">Synthetic Defined (SD) Minimal Yeast Medium</td>
			<td rowspan="3">2% dextrose, 0.67% yeast nitrogen base without amino acids, 0.002% adenine, 0.004% uracil, 0.002% arginine, 0.001% histidine, 0.006% isoleucine, 0.006% leucine, 0.004% lysine, 0.001% methionine, 0.006% phenylalanine, 0.005% threonine, 0.004% tryptophan. For solid (plate) medium, include 2% agar.</td>
			<td>1. Selective medium is prepared by omitting appropriate amino acid(s) or nitrogenous bases.</td>
		</tr>
		<tr>
			<td>2. For convenience, these ingredients may be maintained as concentrated stock solutions as follows. Amino acids may be maintained as 100x stock solution containing all desired amino acids. Yeast nitrogen base may be maintained in a 20x stock solution (13.4%). Dextrose may be maintained in a 40% stock solution. Adenine and uracil may be maintained as 1% stock solutions in 0.1 M NaOH.</td>
		</tr>
		<tr>
			<td>3. Sterilize medium by autoclaving.</td>
		</tr>
		<tr>
			<td rowspan="3">Yeast Extract-Peptone Dextrose (YPD) Rich Yeast Medium</td>
			<td rowspan="3">1% yeast extract, 2% peptone, 2% dextrose (Optional: 0.002% adenine). For solid (plate) medium, include 2% agar.</td>
			<td>1. To prevent the slow growth and red coloration characteristic of particular laboratory yeast strains in the absence (or low abundance) of adenine, adenine may be added to YPD growth medium.</td>
		</tr>
		<tr>
			<td>2. For convenience, some ingredients may be maintained as concentrated stock solutions as follows. Dextrose may be maintained in a 40% stock solution. Adenine may be maintained as a 1% stock solution in 0.1 M NaOH.</td>
		</tr>
		<tr>
			<td>3. Sterilize medium by autoclaving.</td>
		</tr>
		<tr>
			<td>20x Stop Mix</td>
			<td>200 mM sodium azide, 5 mg/ml bovine serum albumin</td>
			<td>Sodium azide is toxic via oral ingestion or dermal contact. Follow manufacturer recommendations when preparing, storing, and handling sodium azide. In the event of accidental exposure, consult material safety data sheet provided by manufacturer. </td>
		</tr>
		<tr>
			<td rowspan="2">20 mg/ml Cycloheximide</td>
			<td rowspan="2"></td>
			<td>1.  Prepare in ethanol. Store at -20 °C.</td>
		</tr>
		<tr>
			<td>2. Cycloheximide is a dermal irritant and is toxic via oral ingestion. Follow manufacturer recommendations when preparing, storing, and handling cycloheximide. In the event of accidental exposure, consult material safety data sheet provided by manufacturer.</td>
		</tr>
		<tr>
			<td>0.2 M Sodium Hydroxide</td>
			<td></td>
			<td>Prepare in water. Sodium hydroxide reacts with glass. Therefore, for long-term storage, 0.2 M sodium hydroxide should be maintained in plastic containers.</td>
		</tr>
		<tr>
			<td rowspan="2">Laemmli Sample Buffer</td>
			<td rowspan="2">2% SDS, 10% glycerol, 5% β-mercaptoethanol, 60 mM Tris HCl pH 6.8, 0.008% bromophenol blue</td>
			<td>1. Laemmli Sample Buffer is often prepared by diluting a more concentrated (e.g., 5x) stock.</td>
		</tr>
		<tr>
			<td>2. The dye bromophenol blue may be added to desired intensity. A "pinch" (very small amount tapped from the edge of a spatula) is typically sufficient.</td>
		</tr>
		<tr>
			<td>Laemmli Running Buffer (5x)</td>
			<td>125 mM Tris, 960 mM glycine, 0.5% SDS</td>
			<td>To prepare 1 L of 1x Laemmli Running Buffer, dilute 1:5 in dH2O.</td>
		</tr>
		<tr>
			<td>Tris Acetate-SDS Transfer Buffer (5x)</td>
			<td>125 mM Tris acetate (pH 8.8), 960 mM glycine, 0.05% SDS</td>
			<td>To prepare 20 L of 1x Tris Acetate-SDS Transfer Buffer, combine 4 L of 5x stock, 4 L of methanol, and 12 L of dH2O.</td>
		</tr>
		<tr>
			<td>10x Tris-Buffered Saline (TBS)</td>
			<td>500 mM Tris, 1.5 M NaCl; pH adjusted to 7.5</td>
			<td>To prepare 1 L of 1x TBS, dilute 1:10 in dH2O. 1x TBS may be supplemented with the detergent Tween-20 and powdered skim milk, as appropriate.</td>
		</tr>
	</tbody>
</table>
Table 1. Solutions Used in this Study.
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Strain Name</td>
			<td>Alias</td>
			<td>Relevant Genotype</td>
			<td>References</td>
		</tr>
		<tr>
			<td rowspan="7">VJY42</td>
			<td rowspan="7">MHY501</td>
			<td>MATα</td>
			<td rowspan="7">Chen et al., 1993</td>
		</tr>
		<tr>
			<td>his3-Δ200</td>
		</tr>
		<tr>
			<td>leu2-3,112 </td>
		</tr>
		<tr>
			<td>ura3-52 </td>
		</tr>
		<tr>
			<td>lys2-801</td>
		</tr>
		<tr>
			<td>trp1-1</td>
		</tr>
		<tr>
			<td>gal2</td>
		</tr>
		<tr>
			<td rowspan="8">VJY47</td>
			<td rowspan="8">YWO55; MHY507</td>
			<td>MATα</td>
			<td rowspan="8">Jungmann et al., 1993; Rubenstein et al., 2012</td>
		</tr>
		<tr>
			<td>his3-Δ200</td>
		</tr>
		<tr>
			<td>leu2-3,112</td>
		</tr>
		<tr>
			<td>ura3-52</td>
		</tr>
		<tr>
			<td>lys2-801</td>
		</tr>
		<tr>
			<td>trp1-1</td>
		</tr>
		<tr>
			<td>gal2</td>
		</tr>
		<tr>
			<td>ubc7Δ::LEU2</td>
		</tr>
		<tr>
			<td rowspan="8">VJY56</td>
			<td rowspan="8">YTX105; MHY1364</td>
			<td>MATα</td>
			<td rowspan="8">Biederer et al., 1997; Ravid et al., 2006</td>
		</tr>
		<tr>
			<td>his3-Δ200</td>
		</tr>
		<tr>
			<td>leu2-3,112</td>
		</tr>
		<tr>
			<td>ura3-52</td>
		</tr>
		<tr>
			<td>lys2-801</td>
		</tr>
		<tr>
			<td>trp1-1</td>
		</tr>
		<tr>
			<td>gal2</td>
		</tr>
		<tr>
			<td>cue1Δ::HIS3</td>
		</tr>
		<tr>
			<td rowspan="8">VJY172</td>
			<td rowspan="8">MHY6199</td>
			<td>MATα</td>
			<td rowspan="8">This study</td>
		</tr>
		<tr>
			<td>his3-Δ200</td>
		</tr>
		<tr>
			<td>leu2-3,112</td>
		</tr>
		<tr>
			<td>ura3-52</td>
		</tr>
		<tr>
			<td>lys2-801</td>
		</tr>
		<tr>
			<td>trp1-1</td>
		</tr>
		<tr>
			<td>gal2</td>
		</tr>
		<tr>
			<td>hrd1Δ::kanMX4</td>
		</tr>
	</tbody>
</table>
Table 2. Yeast Strains Used in this Study. All strains are congenic with MHY500 53. VJY42, VJY47, and VJY56 were described previously 49,53,54. A detailed strain generation and confirmation strategy for VJY172 (prepared for this study) is available upon request.

Watch this Scientific Journal Video about Cycloheximide Chase Analysis of Protein Degradation in Saccharomyces cerevisiae at JoVE.com

Cycloheximide Chase Analysis of Protein Degradation in Saccharomyces cerevisiae

Protein abundance reflects the rates of both protein synthesis and protein degradation. This article describes the use of cycloheximide chase followed by western blotting to analyze protein degradation in the model unicellular eukaryote, Saccharomyces cerevisiae (budding yeast).

Cycloheximide Chase Analysis of Protein Degradation in Saccharomyces cerevisiae

Regulation of protein abundance is crucial to virtually every cellular process. Protein abundance reflects the integration of the rates of protein ...

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28.8K Views.  Ball State University. Protein abundance reflects the rates of both protein synthesis and protein degradation. This article describes the use of cycloheximide chase followed by western blotting to analyze protein degradation in the model unicellular eukaryote, Saccharomyces cerevisiae (budding yeast).

Video: Cycloheximide Chase Analysis of Protein Degradation in Saccharomyces cerevisiae

Evaluation of the Spindle Assembly Checkpoint Integrity in Mouse Oocytes

Aneuploidy is the leading genetic abnormality causing early miscarriage and pregnancy failure in humans. Most errors in chromosome segregation that give rise to aneuploidy occur during meiosis in oocytes, but why oocyte meiosis is error-prone is still not fully understood. During cell division, cells prevent errors in chromosome segregation by activating the spindle assembly checkpoint (SAC). This control mechanism relies on detecting kinetochore (KT)-microtubule (MT) attachments and sensing tension generated by spindle fibers. When KTs are unattached, the SAC is activated and prevents cell-cycle progression. The SAC is activated first by MPS1 kinase, which triggers the recruitment and formation of the mitotic checkpoint complex (MCC), composed of MAD1, MAD2, BUB3, and BUBR1. Then, the MCC diffuses into the cytoplasm and sequesters CDC20, an anaphase-promoting complex/cyclosome (APC/C) activator. Once KTs become attached to microtubules and chromosomes are aligned at the metaphase plate, the SAC is silenced, CDC20 is released, and the APC/C is activated, triggering the degradation of Cyclin B and Securin, thereby allowing anaphase onset. Compared to somatic cells, the SAC in oocytes is not as effective because cells can undergo anaphase despite having unattached KTs. Understanding why the SAC is more permissive and if this permissiveness is one of the causes of chromosome segregation errors in oocytes still needs further investigation. The present protocol describes the three techniques to comprehensively evaluate SAC integrity in mouse oocytes. These techniques include using nocodazole to depolymerize MTs to evaluate the SAC response, tracking SAC silencing by following the kinetics of Securin destruction, and evaluating the recruitment of MAD2 to KTs by immunofluorescence. Together these techniques probe mechanisms needed to produce healthy eggs by providing a complete evaluation of SAC integrity.

Error in chromosome segregation is a common feature in oocytes. Therefore, studying the spindle assembly checkpoint gives important clues about the mechanisms needed to produce healthy eggs. The present protocol describes three complementary assays to evaluate spindle assembly checkpoint integrity in mouse oocytes.

Aneuploidy is the leading genetic abnormality causing early miscarriage and pregnancy failure in humans. Most errors in chromosome segregation that give ...

Developmental Biology

Tuning Degradation to Achieve Specific and Efficient Protein Depletion

The plant auxin binding receptor, TIR1, recognizes proteins containing a specific auxin-inducible degron (AID) motif in the presence of auxin, targeting them for degradation. This system is exploited in many non-plant eukaryotes, such that a target protein, tagged with the AID motif, is degraded upon auxin addition. The level of TIR1 expression is critical; excessive expression leads to degradation of the AID-tagged protein even in the absence of auxin, whereas low expression leads to slow depletion. A &#946;-estradiol-inducible AID system was created, with expression of TIR1 under the control of a &#946;-estradiol inducible promoter. The level of TIR1 is tunable by changing the time of incubation with &#946;-estradiol before auxin addition. This protocol describes how to rapidly deplete a target protein using the AID system. The appropriate &#946;-estradiol incubation time depends on the abundance of the target protein. Therefore, efficient depletion depends on optimal timing that also minimizes auxin-independent depletion.

Here, we present a protocol to effectively and specifically deplete a protein of interest in the yeast Saccharomyces cerevisiae using the &#946;-est AID system.

The plant auxin binding receptor, TIR1, recognizes proteins containing a specific auxin-inducible degron (AID) motif in the presence of auxin, targeting ...

Immunology and Infection

Studying Proteolysis of Cyclin B at the Single Cell Level in Whole Cell Populations

Equal distribution of chromosomes between the two daughter cells during cell division is a prerequisite for guaranteeing genetic stability 1. Inaccuracies during chromosome separation are a hallmark of malignancy and associated with progressive disease 2-4. The spindle assembly checkpoint (SAC) is a mitotic surveillance mechanism that holds back cells at metaphase until every single chromosome has established a stable bipolar attachment to the mitotic spindle1. The SAC exerts its function by interference with the activating APC/C subunit Cdc20 to block proteolysis of securin and cyclin B and thus chromosome separation and mitotic exit. Improper attachment of chromosomes prevents silencing of SAC signaling and causes continued inhibition of APC/CCdc20 until the problem is solved to avoid chromosome missegregation, aneuploidy and malignant growths1.
Most studies that addressed the influence of improper chromosomal attachment on APC/C-dependent proteolysis took advantage of spindle disruption using depolymerizing or microtubule-stabilizing drugs to interfere with chromosomal attachment to microtubules. Since interference with microtubule kinetics can affect the transport and localization of critical regulators, these procedures bear a risk of inducing artificial effects 5.
To study how the SAC interferes with APC/C-dependent proteolysis of cyclin B during mitosis in unperturbed cell populations, we established a histone H2-GFP-based system which allowed the simultaneous monitoring of metaphase alignment of mitotic chromosomes and proteolysis of cyclin B 6.
To depict proteolytic profiles, we generated a chimeric cyclin B reporter molecule with a C-terminal SNAP moiety 6 (Figure 1). In a self-labeling reaction, the SNAP-moiety is able to form covalent bonds with alkylguanine-carriers (SNAP substrate) 7,8 (Figure 1). SNAP substrate molecules are readily available and carry a broad spectrum of different fluorochromes. Chimeric cyclin B-SNAP molecules become labeled upon addition of the membrane-permeable SNAP substrate to the growth medium 7 (Figure 1). Following the labeling reaction, the cyclin B-SNAP fluorescence intensity drops in a pulse-chase reaction-like manner and fluorescence intensities reflect levels of cyclin B degradation 6 (Figure 1). Our system facilitates the monitoring of mitotic APC/C-dependent proteolysis in large numbers of cells (or several cell populations) in parallel. Thereby, the system may be a valuable tool to identify agents/small molecules that are able to interfere with proteolytic activity at the metaphase to anaphase transition. Moreover, as synthesis of cyclin B during mitosis has recently been suggested as an important mechanism in fostering a mitotic block in mice and humans by keeping cyclin B expression levels stable 9,10, this system enabled us to analyze cyclin B proteolysis as one element of a balanced equilibrium 6.

Metaphase to anaphase transition is triggered through anaphase-promoting complex (APC/C)-dependent ubiquitination and subsequent destruction of cyclin B. Here, we established a system which, following pulse-chase labeling, allows monitoring cyclin B proteolysis in entire cell populations and facilitates the detection of interference by the mitotic checkpoint.

Equal distribution of chromosomes between the two daughter cells during cell division is a prerequisite for guaranteeing genetic stability 1. Inaccuracies ...

Reporter-based Growth Assay for Systematic Analysis of Protein Degradation

Protein degradation by the ubiquitin-proteasome system (UPS) is a major regulatory mechanism for protein homeostasis in all eukaryotes. The standard approach to determining intracellular protein degradation relies on biochemical assays for following the kinetics of protein decline. Such methods are often laborious and time consuming and therefore not amenable to experiments aimed at assessing multiple substrates and degradation conditions. As an alternative, cell growth-based assays have been developed, that are, in their conventional format, end-point assays that cannot quantitatively determine relative changes in protein levels.
Here we describe a method that faithfully determines changes in protein degradation rates by coupling them to yeast cell-growth kinetics. The method is based on an established selection system where uracil auxotrophy of URA3-deleted yeast cells is rescued by an exogenously expressed reporter protein, comprised of a fusion between the essential URA3 gene and a degradation determinant (degron). The reporter protein is designed so that its synthesis rate is constant whilst its degradation rate is determined by the degron. As cell growth in uracil-deficient medium is proportional to the relative levels of Ura3, growth kinetics are entirely dependent on the reporter protein degradation.
This method accurately measures changes in intracellular protein degradation kinetics. It was applied to: (a) Assessing the relative contribution of known ubiquitin-conjugating factors to proteolysis (b) E2 conjugating enzyme structure-function analyses (c) Identification and characterization of novel degrons. Application of the degron-URA3-based system transcends the protein degradation field, as it can also be adapted to monitoring changes of protein levels associated with functions of other cellular pathways.

Here we describe a robust biological assay for quantifying the relative rate of proteolysis by the ubiquitin-proteasome system. The assay readout is yeast growth rate in liquid culture, which is dependent on the cellular levels of a reporter protein comprising a degradation signal fused to an essential metabolic marker.

Protein degradation by the ubiquitin-proteasome system (UPS) is a major regulatory mechanism for protein homeostasis in all eukaryotes. The standard ...

Measurement of mRNA Decay Rates in Saccharomyces cerevisiae Using rpb1-1 Strains

mRNA steady state levels vary depending on environmental conditions. Regulation of the steady state accumulation levels of an mRNA ensures that the correct amount of protein is synthesized for the cell&#8217;s specific growth conditions. One approach for measuring mRNA decay rates is inhibiting transcription and subsequently monitoring the disappearance of the already present mRNA. The rate of mRNA decay can then be quantified, and an accurate half-life can be determined utilizing several techniques. In S. cerevisiae, protocols that measure mRNA half-lives have been developed and include inhibiting transcription of mRNA using strains that harbor a temperature sensitive allele of RNA polymerase II, rpb1-1. Other techniques for measuring mRNA half-lives include inhibiting transcription with transcriptional inhibitors such as thiolutin or 1,10-phenanthroline, or alternatively, by utilizing mRNAs that are under the control of a regulatable promoter such as the galactose inducible promoter and the TET-off system. Here, we describe measurement of S. cerevisiae mRNA decay rates using the temperature sensitive allele of RNA polymerase II. This technique can be used to measure mRNA decay rates of individual mRNAs or genome-wide.

Measurement of mRNA Decay Rates in Saccharomyces cerevisiae Using rpb1-1 Strains

The steady state level of specific mRNAs is determined by the rate of synthesis and decay of the mRNA. Genome-wide mRNA degradation rates or the decay rates of specific mRNAs can be measured by determining mRNA half-lives. This protocol focuses on measurement of mRNA decay rates in Saccharomyces cerevisiae.

mRNA steady state levels vary depending on environmental conditions. Regulation of the steady state accumulation levels of an mRNA ensures that the ...

Growth-based Determination and Biochemical Confirmation of Genetic Requirements for Protein Degradation in Saccharomyces cerevisiae

Regulated protein degradation is crucial for virtually every cellular function. Much of what is known about the molecular mechanisms and genetic requirements for eukaryotic protein degradation was initially established in Saccharomyces cerevisiae. Classical analyses of protein degradation have relied on biochemical pulse-chase and cycloheximide-chase methodologies. While these techniques provide sensitive means for observing protein degradation, they are laborious, time-consuming, and low-throughput. These approaches are not amenable to rapid or large-scale screening for mutations that prevent protein degradation. Here, a yeast growth-based assay for the facile identification of genetic requirements for protein degradation is described. In this assay, a reporter enzyme required for growth under specific selective conditions is fused to an unstable protein. Cells lacking the endogenous reporter enzyme but expressing the fusion protein can grow under selective conditions only when the fusion protein is stabilized (i.e. when protein degradation is compromised). In the growth assay described here, serial dilutions of wild-type and mutant yeast cells harboring a plasmid encoding a fusion protein are spotted onto selective and non-selective medium. Growth under selective conditions is consistent with degradation impairment by a given mutation. Increased protein abundance should be biochemically confirmed. A method for the rapid extraction of yeast proteins in a form suitable for electrophoresis and western blotting is also demonstrated. A growth-based readout for protein stability, combined with a simple protocol for protein extraction for biochemical analysis, facilitates rapid identification of genetic requirements for protein degradation. These techniques can be adapted to monitor degradation of a variety of short-lived proteins. In the example presented, the His3 enzyme, which is required for histidine biosynthesis, was fused to Deg1-Sec62. Deg1-Sec62 is targeted for degradation after it aberrantly engages the endoplasmic reticulum translocon. Cells harboring Deg1-Sec62-His3 were able to grow under selective conditions when the protein was stabilized.

Growth-based Determination and Biochemical Confirmation of Genetic Requirements for Protein Degradation in Saccharomyces cerevisiae

This article describes a yeast growth-based assay for the determination of genetic requirements for protein degradation. It also demonstrates a method for rapid extraction of yeast proteins, suitable for western blotting to biochemically confirm degradation requirements. These techniques can be adapted to monitor degradation of a variety of proteins.

Regulated protein degradation is crucial for virtually every cellular function. Much of what is known about the molecular mechanisms and genetic ...

Determination of S-Phase Duration Using 5-Ethynyl-2'-deoxyuridine Incorporation in Saccharomyces cerevisiae

Eukaryotic DNA replication is a highly regulated process that ensures that the genetic blueprint of a cell is correctly duplicated prior to chromosome segregation. As DNA synthesis defects underlie chromosome rearrangements, monitoring DNA replication has become essential to understand the basis of genome instability. Saccharomyces cerevisiae is a classical model to study cell cycle regulation, but key DNA replication parameters, such as the fraction of cells in the S phase or the S-phase duration, are still difficult to determine. This protocol uses short and non-toxic pulses of 5-ethynyl-2'-deoxyuridine (EdU), a thymidine analog, in engineered TK-hENT1 yeast cells, followed by its detection by Click reaction to allow the visualization and quantification of DNA replication with high spatial and temporal resolution at both the single-cell and population levels by microscopy and flow cytometry. This method may identify previously overlooked defects in the S phase and cell cycle progression of yeast mutants, thereby allowing the characterization of new players essential for ensuring genome stability.

Determination of S-Phase Duration Using 5-Ethynyl-2'-deoxyuridine Incorporation in Saccharomyces cerevisiae

We describe two complementary protocols to accurately determine S-phase duration in S. cerevisiae using EdU, a thymidine analog, which is incorporated in vivo and detected using Click chemistry by microscopy and flow cytometry. It allows for the easy characterization of the duration of DNA replication and overlooked replication defects in mutants.

Eukaryotic DNA replication is a highly regulated process that ensures that the genetic blueprint of a cell is correctly duplicated prior to chromosome ...

Use of Time-Lapse Microscopy and Stage-Specific Nuclear Depletion of Proteins to Study Meiosis in S. cerevisiae

Time-lapse fluorescence microscopy has revolutionized the understanding of meiotic cell-cycle events by providing temporal and spatial data that is often not seen by imaging fixed cells. Budding yeast has proved to be an important model organism to study meiotic chromosome segregation because many meiotic genes are highly conserved. Time-lapse microscopy of meiosis in budding yeast allows the monitoring of different meiotic mutants to show how the mutation disrupts meiotic processes. However, many proteins function at multiple points in meiosis. The use of loss-of-function or meiotic null mutants can therefore disrupt an early process, blocking or disturbing the later process and making it difficult to determine the phenotypes associated with each individual role. To circumvent this challenge, this protocol describes how the proteins can be conditionally depleted from the nucleus at specific stages of meiosis while monitoring meiotic events using time-lapse microscopy. Specifically, this protocol describes how the cells are synchronized in prophase I, how the anchor away technique is used to deplete proteins from the nucleus at specific meiotic stages, and how time-lapse imaging is used to monitor meiotic chromosome segregation. As an example of the usefulness of the technique, the kinetochore protein Ctf19 was depleted from the nucleus at different time points during meiosis, and the number of chromatin masses was analyzed at the end of meiosis II. Overall, this protocol can be adapted to deplete different nuclear proteins from the nucleus while monitoring the meiotic divisions.

Use of Time-Lapse Microscopy and Stage-Specific Nuclear Depletion of Proteins to Study Meiosis in S. cerevisiae

Time-lapse microscopy is a valuable tool for studying meiosis in budding yeast. This protocol describes a method that combines cell-cycle synchronization, time-lapse microscopy, and conditional depletion of a target protein to demonstrate how to study the function of a specific protein during meiotic chromosome segregation.

Time-lapse fluorescence microscopy has revolutionized the understanding of meiotic cell-cycle events by providing temporal and spatial data that is often ...

An Introduction to Saccharomyces cerevisiae

Saccharomyces cerevisiae (commonly known as baker&rsquo;s yeast) is a single-celled eukaryote that is frequently used in scientific research. S. cerevisiae is an attractive model organism due to the fact that its genome has been sequenced, its genetics are easily manipulated, and it is very easy to maintain in the lab. Because many yeast proteins are similar in sequence and function to those found in other organisms, studies performed in yeast can help us to determine how a particular gene or protein functions in higher eukaryotes (including humans).
This video provides an introduction to the biology of this model organism, how it was discovered, and why labs all over the world have selected it as their model of choice. Previous studies performed in S. cerevisiae that have contributed to our understanding of important cellular processes such as the cell cycle, aging, and cell death are also discussed. Finally, the video describes some of the many ways in which yeast cells are put to work in modern scientific research, including protein purification and the study of DNA repair mechanisms and other cellular processes related to Alzheimer&rsquo;s and Parkinson&rsquo;s diseases.

Saccharomyces cerevisiae Yeast as a Model Organism

Saccharomyces cerevisiae (commonly known as baker&rsquo;s yeast) is a single-celled eukaryote that is frequently used in scientific research.  S. ...

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Misfolding-Prone Protein Degradation Assay: A Technique to Monitor Misfolded Protein Degradation Using Cycloheximide Treatment and Detergent Fractionation

Source: Guo, L. et al., <a href="https://app-jove-com.remotexs.ntu.edu.sg/v/54266">Assays for the Degradation of Misfolded Proteins in Cells.</a> J. Vis. Exp. (2016).
This video describes a degradation assay for misfolded proteins using cycloheximide treatment along with detergent fractionation. This method aids in studying the dynamics of misfolded proteins and uncovering the in-depth mechanisms of protein turnover.

Source: Guo, L. et al., Assays for the Degradation of Misfolded Proteins in Cells. J. Vis. Exp. (2016).
This video describes a degradation assay for ...

Cycloheximide Chase Analysis of Protein Degradation in Saccharomyces cerevisiae

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