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Architecture and control of exocytosis and endocytosis in excitable cells

可兴奋细胞胞吐作用和内吞作用的结构和控制

基本信息

批准号：
10253854
负责人：
Justin Taraska
金额：
$ 184.62万
依托单位：
NATIONAL HEART, LUNG, AND BLOOD INSTITUTE
依托单位国家：
美国
项目类别：
财政年份：
资助国家：
美国
起止时间：
至
项目状态：
未结题

来源：
https://reporter.nih.gov/project-details/10253854
关键词：
3-Dimensional Architecture Beta Cell Biochemistry Cancer Intervention Cell membrane Cells Cellular biology Clathrin Clathrin-Coated Vesicles Cryoelectron Microscopy Cytoplasmic Granules Data Development Disease Docking Dynamin Electron Microscopy Electrophysiology (science)Endocrine Endocytosis Environment Eukaryotic Cell Event Exocytosis Extracellular Space Generations Genetic Goals Guanosine Triphosphate Hela Cells Heterogeneity Human Human Biology Hydrolysis Image Image Analysis Individual Kinetics Link Lipids Location Mammalian Cell Maps Matrix Metalloproteinases Mediating Membrane Membrane Fusion Membrane Proteins Microscopy Modeling Molecular Movement Mutation Neck Neurons Neurosecretory Systems Organelles Pathway interactions Peptides Permeability Platinum Point Mutation Polymers Population Positioning Attribute Process Protein Dynamics Proteins Regulation Resolution Retrieval Role Shapes Signal Pathway Signal Transduction Site Structural Models Structure Structure-Activity Relationship Synapses System Testing Thinness Time Total Internal Reflection Fluorescent Transmission Electron Microscopy Vesicle Work amphiphysin cancer cell cancer invasiveness cell motility coated pit flexibility fluorescence imaging genetic regulatory protein geometric structure imaging modality imaging study light microscopy live cell imaging membrane model microscopic imaging microvesicles multimodality nano nanoscale novel physical model polarized cell protein complex recruit small molecule targeted treatment tool trafficking vesicle transport vesicular release

项目摘要

Dozens of proteins control the docking and fusion of exocytic vesicles in human cells. The identity and roles of many of these proteins have been assigned through a combination of genetics, biochemistry, and electrophysiology. However, the spatial organization, heterogeneity, regulation, and dynamics of these proteins have not yet been determined. Finding this organization is key to understanding how proteins regulate membrane trafficking systems in healthy cells and might malfunction in diseases. Thus, we aimed to map key proteins that act during membrane fusion and fission at the plasma membrane. To accomplish this, we developed a combination of high-throughput live cell imaging, super-resolution fluorescence imaging, and electron microscopy to directly visualize organelles. Through this multi-modal approach the location, dynamics, and occupancy of individual proteins were determined at specific populations of vesicles in cells. This allowed us to determine the fundamental organization of the vesicle systems and how specific molecular components responsible for vesicle movement, docking, fusion, and the subsequent recapture of material assemble together in time and space at the plasma membrane of cells. First, with TIRF microscopy and high-throughput image analysis we developed a universal map of proteins that control exocytosis and provide a global network level analysis of vesicle fusion events. We were able to identify unique classes of key regulatory molecules that strongly associate with the vast majority of exocytic vesicles in both cultured neuroendocrine PC12, chromaffin, and INS1 beta cells. To determine the local dynamics of these molecules at single sites of exocytosis we imaged signal changes of proteins at the exact moment of fusion. In these studies we discovered an unexpected recruitment of several important endocytic proteins to sites of both synaptic-like microvesicle fusion and large dense-core granule fusion. These molecules include the regulatory proteins dynamin, amphiphysin, syndapin, and endophilin. We further discovered that mutations of several of these proteins altered the kinetics of vesicle membrane protein release into the plasma membrane. Our hypothesis is that these proteins (dynamin, syndapin, amphiphysin, and endophilin) regulate the dilation, permeability, or closure of the fusion pore to control the amount of membrane-bound cargo released during single exocytic fusion events. This would allow excitable cells to modulate the amount of material released during even single exocytic fusion events. Aside from classical exocytic vesicles in endocrine cells and neurons, cancer cells release proteins to regulate their motility and invasiveness. We next worked on a collaborative project to image the dynamic recruitment of proteins to vesicles that release matrix metalloproteinases (MMPs) in invasive cancer cells. With live cell imaging and analysis, dozens of proteins were dynamically mapped to vesicles that released MMPs into the extracellular space. These studies helped define the regulation and control of vesicle fusion in cancer cells and provides new and important targets for the therapeutic intervention of cancer. After exocytosis, with live cell imaging we discovered that vesicle material is captured on a dense network of pre-formed clathrin-coated endocytic structures following exocytosis. Despite the identification of many components of clathrin-mediated endocytosis, a structural understanding of how these molecules come together to build and retrieve material from the plasma membrane during endocytosis is likewise incomplete. In our next aim we determined the nanoscale structure of clathrin-coated vesicles responsible for endocytosis in mammalian cells. By understanding how proteins that have been functionally linked to endocytosis assemble together we can place decades of biochemistry, cell biology, and genetics into a physical model of membrane retrieval. These data are key for understanding how endocytosis is regulated in human cells. To determine the nanoscale structure of endocytic sites, we developed a novel super-resolution correlative light and electron microscopy imaging (CLEM) method. This allows us to image the nanometer-scale location of proteins in the context of their local cellular environment. Specifically, we developed a robust pipeline for imaging the plasma membrane of cells with super-resolution localization microscopy and transmission electron microscopy (TEM) of platinum replicas. In these studies we imaged the position of endocytic proteins at single clathrin-coated structures. This generated a comprehensive molecular architecture of endocytosis with nano-precision in human Hela cells. From this work, we discovered that endocytic proteins distribute into distinct spatial zones (rings) in relation to the edge of the clathrin lattice. The presence or concentrations of specific proteins within these rings change at distinct stages of organelle development. We propose that endocytosis is driven by the recruitment, reorganization, and loss of proteins within these partitioned nanoscale zones. In total, these studies are allowing us to build structural models for how proteins are organized at single organelles to regulate endocytosis, a key process for all eukaryotic cells. Clathrin-coated pits dynamically assemble and disassemble at the membrane of mammalian cells. Models of how clathrin coats curve have been controversial. Specifically, some models propose that clathrin can only grow as a curved lattice while others propose that clathrin first assembles as a fully formed flat lattice that later curves into a sphere. We tested these models in two collaborative projects by imaging growing clathrin structures with both live cell polarized total internal reflection microscopy (pTIRF) and super-resolution EM correlative imaging. In these studies we watched single pits curve at the plasma membrane and related these observations to structures observed in EM. Our work demonstrated that the pathway for curvature is heterogenous. First, many clathrin sites form as small curved structures, others grow partially flat and then begin to curve, and some grow to their full size and bend. Thus, cells control the pathway of membrane curvature with multiple mechanisms of curvature generation in the lattice. In an effort to better understand how cells specifically regulate the assembly and curvature of single clathrin-coated endocytic structures we have been examining the geometric structural transitions in the clathrin-coat with high resolution 3D and CryoEM microscopy. To accomplish this, platinum-replica EM has been used to track and examine in detail how the lattices assemble and dynamically rearrange in hundreds of different cells. These studies are showing that the clathrin lattice is dynamic and flexible and capable of assembling first as a flat lattice that then uses geometric transitions in the individual clathrin subunits to drive curvature. These structural transitions drive coat reassembly to re-shape a transport vesicle and control cellular signaling pathways. Dynamin assembles into helical polymers around the necks of vesicles to cut the thin membranous neck connecting clathrin-coated pits to the membrane. This process is driven by the hydrolysis of GTP. With super-resolution and EM imaging we have mapped the nanoscale location of dynamin at single clathrin sites. We next worked on a collaborative project to solve the atomic CryoEM structure of dynamin assembled on lipid tubules. In these studies, we found specific point-mutations within Dynamin that block its function. These mutations helped us understand the structure-function relationship in the dynamin protein complex responsible for its essential role in the cell.