Conditional control of gene expression allows an experimenter to investigate many aspects of a gene's function. In the model organism
- NSF-PAR ID:
- 10424939
- Date Published:
- Journal Name:
- The Twenty-first ACM Workshop on Hot Topics in Networks (HotNets 2022)
- Page Range / eLocation ID:
- 221 to 227
- Format(s):
- Medium: X
- Sponsoring Org:
- National Science Foundation
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Abstract Saccharomyces cerevisiae , a number of methods to control gene expression are widely practiced, including induction by metabolites, small molecules, and even light. However, all current methods suffer from at least one of a set of drawbacks, including need for specialized growth conditions, leaky expression, or requirement of specialized equipment. Here we describe protocols using two transformations to construct strains that carry a new controller in which all these drawbacks are overcome. In these strains, the expression of a controlled gene of interest is repressed by the bacterial repressor TetR and induced by anhydrotetracycline. TetR also regulates its own expression, creating an autorepression loop. This autorepression allows tight control of gene expression and protein dosage with low cell‐to‐cell variation in expression. A second repressor, TetR‐Tup1, prevents any leaky expression. We also present a protocol showing a particular workhorse application of such strains to generate synchronized cell populations. We turn off expression of the cell cycle regulatorCDC20 completely, arresting the cell population, and then we turn it back on so that the synchronized cells resume cell cycle progression. This control system can be applied to any endogenous or exogenous gene for precise expression. © 2023 Wiley Periodicals LLC.Basic Protocol 1 : Generating a parent WTC846strainBasic Protocol 2 : Generating a WTC846strain with controlled expression of the targeted geneAlternate Protocol : CRISPR‐mediated promoter replacementBasic Protocol 3 : Cell cycle synchronization/arrest and release using the WTC846‐K3::CDC20 strain -
The shared nature of the wireless medium induces contention between data transport and backward signaling, such as acknowledgement. The current way of TCP acknowledgment induces control overhead which is counter-productive for TCP performance especially in wireless local area network (WLAN) scenarios.In this paper, we present a new acknowledgement called TACK ("Tame ACK"), as well as its TCP implementation TCP-TACK. TCP-TACK works on top of commodity WLAN, delivering high wireless transport goodput with minimal control overhead in the form of ACKs, without any hardware modification. To minimize ACK frequency, TACK abandons the legacy received-packet-driven ACK. Instead, it balances byte-counting ACK and periodic ACK so as to achieve a controlled ACK frequency. Evaluation results show that TCP-TACK achieves significant advantages over legacy TCP in WLAN scenarios due to less contention between data packets and ACKs. Specifically, TCP-TACK reduces over 90% of ACKs and also obtains an improvement of ~ 28% on good-put. We further find it performs equally well as high-speed TCP variants in wide area network (WAN) scenarios, this is attributed to the advancements of the TACK-based protocol design in loss recovery, round-trip timing, and send rate control.more » « less
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Abstract Visualization of gene products in
Caenorhabditis elegans has provided insights into the molecular and biological functions of many novel genes in their native contexts. Single‐molecule fluorescencein situ hybridization (smFISH) and immunofluorescence (IF) enable the visualization of the abundance and localization of mRNAs and proteins, respectively, allowing researchers to ultimately elucidate the localization, dynamics, and functions of the corresponding genes. Whereas both smFISH and immunofluorescence have been foundational techniques in molecular biology, each protocol poses challenges for use in theC. elegans embryo. smFISH protocols suffer from high initial costs and can photobleach rapidly, and immunofluorescence requires technically challenging permeabilization steps and slide preparation. Most importantly, published smFISH and IF protocols have predominantly been mutually exclusive, preventing the exploration of relationships between an mRNA and a relevant protein in the same sample. Here, we describe protocols to perform immunofluorescence and smFISH inC. elegans embryos either in sequence or simultaneously. We also outline the steps to perform smFISH or immunofluorescence alone, including several improvements and optimizations to existing approaches. These protocols feature improved fixation and permeabilization steps to preserve cellular morphology while maintaining probe and antibody accessibility in the embryo, a streamlined, in‐tube approach for antibody staining that negates freeze‐cracking, a validated method to perform the cost‐reducing single molecule inexpensive FISH (smiFISH) adaptation, slide preparation using empirically determined optimal antifade products, and straightforward quantification and data analysis methods. Finally, we discuss tricks and tips to help the reader optimize and troubleshoot individual steps in each protocol. Together, these protocols simplify existing workflows for single‐molecule RNA and protein detection. Moreover, simultaneous, high‐resolution imaging of proteins and RNAs of interest will permit analysis, quantification, and comparison of protein and RNA distributions, furthering our understanding of the relationship between RNAs and their protein products or cellular markers in early development. © 2021 Wiley Periodicals LLC.Basic Protocol 1 : Sequential immunofluorescence and single‐molecule fluorescencein situ hybridizationAlternate Protocol : Abbreviated protocol for simultaneous immunofluorescence and single‐molecule fluorescencein situ hybridizationBasic Protocol 2 : Simplified immunofluorescence inC. elegans embryosBasic Protocol 3 : Single‐molecule fluorescencein situ hybridization or single‐molecule inexpensive fluorescencein situ hybridization -
Abstract Fluorescence fluctuation spectroscopy (FFS) encompasses a bevy of techniques that involve analyzing fluorescence intensity fluctuations occurring due to fluorescently labeled molecules diffusing in and out of a microscope's focal region. Statistical analysis of these fluctuations may reveal the oligomerization (i.e., association) state of said molecules. We have recently developed a new FFS‐based method, termed Two‐Dimensional Fluorescence Intensity Fluctuation (2D FIF) spectrometry, which provides quantitative information on the size and stability of protein oligomers as a function of receptor concentration. This article describes protocols for employing FIF spectrometry to quantify the oligomerization of a membrane protein of interest, with specific instructions regarding cell preparation, image acquisition, and analysis of images given in detail. Application of the FIF Spectrometry Suite, a software package designed for applying FIF analysis on fluorescence images, is emphasized in the protocol. Also discussed in detail is the identification, removal, and/or analysis of inhomogeneous regions of the membrane that appear as bright spots. The 2D FIF approach is particularly suited to assess the effects of agonists and antagonists on the oligomeric size of membrane receptors of interest. © 2022 Wiley Periodicals LLC.
Basic Protocol 1 : Preparation of live cells expressing protein constructsBasic Protocol 2 : Image acquisition and noise correctionBasic Protocol 3 : Drawing and segmenting regions of interestBasic Protocol 4 : Calculating the molecular brightness and concentration of individual image segmentsBasic Protocol 5 : Combining data subsets using a manual procedure (Optional)Alternate Protocol 1 : Combining data subsets using the advanced FIF spectrometry suite (Optional; alternative to Basic Protocol 5)Basic Protocol 6 : Performing meta‐analysis of brightness spectrogramsAlternate Protocol 2 : Performing meta‐analysis of brightness spectrograms (alternative to Basic Protocol 6)Basic Protocol 7 : Spot extraction and analysis using a manual procedure or by writing a program (Optional)Alternate Protocol 3 : Automated spot extraction and analysis (Optional; alternative to Protocol 7)Support Protocol : Monomeric brightness determination -
Abstract Protein activity is generally functionally integrated and spatially restricted to key locations within the cell. Knocksideways experiments allow researchers to rapidly move proteins to alternate or ectopic regions of the cell and assess the resultant cellular response. Briefly, individual proteins to be tested using this approach must be modified with moieties that dimerize under treatment with rapamycin to promote the experimental spatial relocalizations. CRISPR technology enables researchers to engineer modified protein directly in cells while preserving proper protein levels because the engineered protein will be expressed from endogenous promoters. Here we provide straightforward instructions to engineer tagged, rapamycin‐relocalizable proteins in cells. The protocol is described in the context of our work with the microtubule depolymerizer MCAK/Kif2C, but it is easily adaptable to other genes and alternate tags such as degrons, optogenetic constructs, and other experimentally useful modifications. Off‐target effects are minimized by testing for the most efficient target site using a split‐GFP construct. This protocol involves no proprietary kits, only plasmids available from repositories (such as addgene.org). Validation, relocalization, and some example novel discoveries obtained working with endogenous protein levels are described. A graduate student with access to a fluorescence microscope should be able to prepare engineered cells with spatially controllable endogenous protein using this protocol. © 2023 The Authors. Current Protocols published by Wiley Periodicals LLC.
Basic Protocol 1 : Choosing a target site for gene modificationBasic Protocol 2 : Design of gRNA(s) for targeted gene modificationBasic Protocol 3 : Split‐GFP test for target efficiencyBasic Protocol 4 : Design of the recombination template and analytical primersSupport Protocol 1 : Design of primers for analytical PCRBasic Protocol 5 : Transfection, isolation, and validation of engineered cellsSupport Protocol 2 : Stable transfection of engineered cells with binding partners