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Weakly HMJ, Keller SL. Coupling liquid phases in 3D condensates and 2D membranes: Successes, challenges, and tools. Biophys J 2024; 123:1329-1341. [PMID: 38160256 PMCID: PMC11163299 DOI: 10.1016/j.bpj.2023.12.023] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/21/2023] [Revised: 12/05/2023] [Accepted: 12/26/2023] [Indexed: 01/03/2024] Open
Abstract
This review describes the major experimental challenges researchers meet when attempting to couple phase separation between membranes and condensates. Although it is well known that phase separation in a 2D membrane could affect molecules capable of forming a 3D condensate (and vice versa), few researchers have quantified the effects to date. The scarcity of these measurements is not due to a lack of intense interest or effort in the field. Rather, it reflects significant experimental challenges in manipulating coupled membranes and condensates to yield quantitative values. These challenges transcend many molecular details, which means they impact a wide range of systems. This review highlights recent exciting successes in the field, and it lays out a comprehensive list of tools that address potential pitfalls for researchers who are considering coupling membranes with condensates.
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Affiliation(s)
- Heidi M J Weakly
- Department of Chemistry, University of Washington - Seattle, Seattle, Washington
| | - Sarah L Keller
- Department of Chemistry, University of Washington - Seattle, Seattle, Washington.
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2
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Govey-Scotland J, Johnstone L, Myant C, Friddin MS. Towards skin-on-a-chip for screening the dermal absorption of cosmetics. LAB ON A CHIP 2023; 23:5068-5080. [PMID: 37938128 DOI: 10.1039/d3lc00691c] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 11/09/2023]
Abstract
Over the past few decades, there have been increasing global efforts to limit or ban the use of animals for testing cosmetic products. This ambition has been at the heart of international endeavours to develop new in vitro and animal-free approaches for assessing the safety of cosmetics. While several of these new approach methodologies (NAMs) have been approved for assessing different toxicological endpoints in the UK and across the EU, there remains an absence of animal-free methods for screening for dermal absorption; a measure that assesses the degree to which chemical substances can become systemically available through contact with human skin. Here, we identify some of the major technical barriers that have impacted regulatory recognition of an in vitro skin model for this purpose and propose how these could be overcome on-chip using artificial cells engineered from the bottom-up. As part of our future perspective, we suggest how this could be realised using a digital biomanufacturing pipeline that connects the design, microfluidic generation and 3D printing of artificial cells into user-crafted synthetic tissues. We highlight milestone achievements towards this goal, identify future challenges, and suggest how the ability to engineer animal-free skin models could have significant long-term consequences for dermal absorption screening, as well as for other applications.
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Affiliation(s)
- Jessica Govey-Scotland
- Dyson School of Design Engineering, Imperial College London, Exhibition Road, South Kensington, SW7 2AZ, London, UK.
- Institute for Molecular Sciences and Engineering, Imperial College London, Exhibition Road, South Kensington, SW7 2AZ, London, UK
| | - Liam Johnstone
- Office for Product Safety and Standards, 1 Victoria Street, SW1H 0ET, London, UK
| | - Connor Myant
- Dyson School of Design Engineering, Imperial College London, Exhibition Road, South Kensington, SW7 2AZ, London, UK.
| | - Mark S Friddin
- Dyson School of Design Engineering, Imperial College London, Exhibition Road, South Kensington, SW7 2AZ, London, UK.
- Institute for Molecular Sciences and Engineering, Imperial College London, Exhibition Road, South Kensington, SW7 2AZ, London, UK
- fabriCELL, Imperial College London and Kings College London, London, UK
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3
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Jayaram AK, Pappa AM, Ghosh S, Manzer ZA, Traberg WC, Knowles TPJ, Daniel S, Owens RM. Biomembranes in bioelectronic sensing. Trends Biotechnol 2021; 40:107-123. [PMID: 34229865 DOI: 10.1016/j.tibtech.2021.06.001] [Citation(s) in RCA: 8] [Impact Index Per Article: 2.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/25/2021] [Revised: 06/01/2021] [Accepted: 06/03/2021] [Indexed: 12/14/2022]
Abstract
Cell membranes are integral to the functioning of the cell and are therefore key to drive fundamental understanding of biological processes for downstream applications. Here, we review the current state-of-the-art with respect to biomembrane systems and electronic substrates, with a view of how the field has evolved towards creating biomimetic conditions and improving detection sensitivity. Of particular interest are conducting polymers, a class of electroactive polymers, which have the potential to create the next step-change for bioelectronics devices. Lastly, we discuss the impact these types of devices could have for biomedical applications.
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Affiliation(s)
- A K Jayaram
- Centre for Misfolding Diseases, Yusuf Hamied Department of Chemistry, University of Cambridge, CB2 1EW, Cambridge, UK; Cavendish Laboratory, Department of Physics, University of Cambridge, JJ Thomson Avenue, Cambridge CB3 0JH, UK
| | - A M Pappa
- Department of Chemical Engineering and Biotechnology, University of Cambridge, Philippa Fawcett Drive, CB30AS Cambridge, UK
| | - S Ghosh
- RF Smith School of Chemical and Biomolecular Engineering, Cornell University, Olin Hall, Ithaca, NY 14850, USA
| | - Z A Manzer
- RF Smith School of Chemical and Biomolecular Engineering, Cornell University, Olin Hall, Ithaca, NY 14850, USA
| | - W C Traberg
- Department of Chemical Engineering and Biotechnology, University of Cambridge, Philippa Fawcett Drive, CB30AS Cambridge, UK
| | - T P J Knowles
- Centre for Misfolding Diseases, Yusuf Hamied Department of Chemistry, University of Cambridge, CB2 1EW, Cambridge, UK; Cavendish Laboratory, Department of Physics, University of Cambridge, JJ Thomson Avenue, Cambridge CB3 0JH, UK
| | - S Daniel
- RF Smith School of Chemical and Biomolecular Engineering, Cornell University, Olin Hall, Ithaca, NY 14850, USA
| | - R M Owens
- Department of Chemical Engineering and Biotechnology, University of Cambridge, Philippa Fawcett Drive, CB30AS Cambridge, UK.
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4
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Friddin MS, Bolognesi G, Salehi-Reyhani A, Ces O, Elani Y. Direct manipulation of liquid ordered lipid membrane domains using optical traps. Commun Chem 2019. [DOI: 10.1038/s42004-018-0101-4] [Citation(s) in RCA: 11] [Impact Index Per Article: 1.8] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/29/2022] Open
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Trantidou T, Friddin MS, Salehi-Reyhani A, Ces O, Elani Y. Droplet microfluidics for the construction of compartmentalised model membranes. LAB ON A CHIP 2018; 18:2488-2509. [PMID: 30066008 DOI: 10.1039/c8lc00028j] [Citation(s) in RCA: 65] [Impact Index Per Article: 9.3] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/22/2023]
Abstract
The design of membrane-based constructs with multiple compartments is of increasing importance given their potential applications as microreactors, as artificial cells in synthetic-biology, as simplified cell models, and as drug delivery vehicles. The emergence of droplet microfluidics as a tool for their construction has allowed rapid scale-up in generation throughput, scale-down of size, and control over gross membrane architecture. This is true on several levels: size, level of compartmentalisation and connectivity of compartments can all be programmed to various degrees. This tutorial review explains and explores the reasons behind this. We discuss microfluidic strategies for the generation of a family of compartmentalised systems that have lipid membranes as the basic structural motifs, where droplets are either the fundamental building blocks, or are precursors to the membrane-bound compartments. We examine the key properties associated with these systems (including stability, yield, encapsulation efficiency), discuss relevant device fabrication technologies, and outline the technical challenges. In doing so, we critically review the state-of-play in this rapidly advancing field.
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Affiliation(s)
- T Trantidou
- Department of Chemistry, Imperial College London, London, SW7 2AZ, UK.
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6
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Booth MJ, Restrepo Schild V, Downs FG, Bayley H. Functional aqueous droplet networks. MOLECULAR BIOSYSTEMS 2018; 13:1658-1691. [PMID: 28766622 DOI: 10.1039/c7mb00192d] [Citation(s) in RCA: 44] [Impact Index Per Article: 6.3] [Reference Citation Analysis] [Abstract] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 11/21/2022]
Abstract
Droplet interface bilayers (DIBs), comprising individual lipid bilayers between pairs of aqueous droplets in an oil, are proving to be a useful tool for studying membrane proteins. Recently, attention has turned to the elaboration of networks of aqueous droplets, connected through functionalized interface bilayers, with collective properties unachievable in droplet pairs. Small 2D collections of droplets have been formed into soft biodevices, which can act as electronic components, light-sensors and batteries. A substantial breakthrough has been the development of a droplet printer, which can create patterned 3D droplet networks of hundreds to thousands of connected droplets. The 3D networks can change shape, or carry electrical signals through defined pathways, or express proteins in response to patterned illumination. We envisage using functional 3D droplet networks as autonomous synthetic tissues or coupling them with cells to repair or enhance the properties of living tissues.
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Affiliation(s)
- Michael J Booth
- Department of Chemistry, University of Oxford, 12 Mansfield Road, Oxford, OX1 3TA, UK.
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7
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Visualization of lipid directed dynamics of perilipin 1 in human primary adipocytes. Sci Rep 2017; 7:15011. [PMID: 29118433 PMCID: PMC5678101 DOI: 10.1038/s41598-017-15059-4] [Citation(s) in RCA: 33] [Impact Index Per Article: 4.1] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/27/2017] [Accepted: 10/19/2017] [Indexed: 12/20/2022] Open
Abstract
Perilipin 1 is a lipid droplet coating protein known to regulate lipid metabolism in adipocytes by serving as a physical barrier as well as a recruitment site for lipases to the lipid droplet. Phosphorylation of perilipin 1 by protein kinase A rapidly initiates lipolysis, but the detailed mechanism on how perilipin 1 controls lipolysis is unknown. Here, we identify specific lipid binding properties of perilipin 1 that regulate the dynamics of lipolysis in human primary adipocytes. Cellular imaging combined with biochemical and biophysical analyses demonstrate that perilipin 1 specifically binds to cholesteryl esters, and that their dynamic properties direct segregation of perilipin 1 into topologically distinct micro domains on the lipid droplet. Together, our data points to a simple unifying mechanism that lipid assembly and segregation control lipolysis in human primary adipocytes.
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Taylor GJ, Heberle FA, Seinfeld JS, Katsaras J, Collier CP, Sarles SA. Capacitive Detection of Low-Enthalpy, Higher-Order Phase Transitions in Synthetic and Natural Composition Lipid Membranes. LANGMUIR : THE ACS JOURNAL OF SURFACES AND COLLOIDS 2017; 33:10016-10026. [PMID: 28810118 DOI: 10.1021/acs.langmuir.7b02022] [Citation(s) in RCA: 27] [Impact Index Per Article: 3.4] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 06/07/2023]
Abstract
In-plane lipid organization and phase separation in natural membranes play key roles in regulating many cellular processes. Highly cooperative, first-order phase transitions in model membranes consisting of few lipid components are well understood and readily detectable via calorimetry, densitometry, and fluorescence. However, far less is known about natural membranes containing numerous lipid species and high concentrations of cholesterol, for which thermotropic transitions are undetectable by the above-mentioned techniques. We demonstrate that membrane capacitance is highly sensitive to low-enthalpy thermotropic transitions taking place in complex lipid membranes. Specifically, we measured the electrical capacitance as a function of temperature for droplet interface bilayer model membranes of increasing compositional complexity, namely, (a) a single lipid species, (b) domain-forming ternary mixtures, and (c) natural brain total lipid extract (bTLE). We observed that, for single-species lipid bilayers and some ternary compositions, capacitance exhibited an abrupt, temperature-dependent change that coincided with the transition detected by other techniques. In addition, capacitance measurements revealed transitions in mixed-lipid membranes that were not detected by the other techniques. Most notably, capacitance measurements of bTLE bilayers indicated a transition at ∼38 °C not seen with any other method. Likewise, capacitance measurements detected transitions in some well-studied ternary mixtures that, while known to yield coexisting lipid phases, are not detected with calorimetry or densitometry. These results indicate that capacitance is exquisitely sensitive to low-enthalpy membrane transitions because of its sensitivity to changes in bilayer thickness that occur when lipids and excess solvent undergo subtle rearrangements near a phase transition. Our findings also suggest that heterogeneity confers stability to natural membranes that function near transition temperatures by preventing unwanted defects and macroscopic demixing associated with high-enthalpy transitions commonly found in simpler mixtures.
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Affiliation(s)
- Graham J Taylor
- Department of Mechanical, Aerospace, and Biomedical Engineering, and §Department of Physics and Astronomy, The University of Tennessee , Knoxville, Tennessee 37996, United States
- Joint Institute for Biological Sciences, ⊥Biology and Soft Matter Division, #Shull Wollan Center-A Joint Center for Neutron Sciences, and ∇Center for Nanophase Materials Sciences, Oak Ridge National Laboratory , Oak Ridge, Tennessee 37831, United States
| | - Frederick A Heberle
- Department of Mechanical, Aerospace, and Biomedical Engineering, and §Department of Physics and Astronomy, The University of Tennessee , Knoxville, Tennessee 37996, United States
- Joint Institute for Biological Sciences, ⊥Biology and Soft Matter Division, #Shull Wollan Center-A Joint Center for Neutron Sciences, and ∇Center for Nanophase Materials Sciences, Oak Ridge National Laboratory , Oak Ridge, Tennessee 37831, United States
| | - Jason S Seinfeld
- Department of Mechanical, Aerospace, and Biomedical Engineering, and §Department of Physics and Astronomy, The University of Tennessee , Knoxville, Tennessee 37996, United States
- Joint Institute for Biological Sciences, ⊥Biology and Soft Matter Division, #Shull Wollan Center-A Joint Center for Neutron Sciences, and ∇Center for Nanophase Materials Sciences, Oak Ridge National Laboratory , Oak Ridge, Tennessee 37831, United States
| | - John Katsaras
- Department of Mechanical, Aerospace, and Biomedical Engineering, and §Department of Physics and Astronomy, The University of Tennessee , Knoxville, Tennessee 37996, United States
- Joint Institute for Biological Sciences, ⊥Biology and Soft Matter Division, #Shull Wollan Center-A Joint Center for Neutron Sciences, and ∇Center for Nanophase Materials Sciences, Oak Ridge National Laboratory , Oak Ridge, Tennessee 37831, United States
| | - C Patrick Collier
- Department of Mechanical, Aerospace, and Biomedical Engineering, and §Department of Physics and Astronomy, The University of Tennessee , Knoxville, Tennessee 37996, United States
- Joint Institute for Biological Sciences, ⊥Biology and Soft Matter Division, #Shull Wollan Center-A Joint Center for Neutron Sciences, and ∇Center for Nanophase Materials Sciences, Oak Ridge National Laboratory , Oak Ridge, Tennessee 37831, United States
| | - Stephen A Sarles
- Department of Mechanical, Aerospace, and Biomedical Engineering, and §Department of Physics and Astronomy, The University of Tennessee , Knoxville, Tennessee 37996, United States
- Joint Institute for Biological Sciences, ⊥Biology and Soft Matter Division, #Shull Wollan Center-A Joint Center for Neutron Sciences, and ∇Center for Nanophase Materials Sciences, Oak Ridge National Laboratory , Oak Ridge, Tennessee 37831, United States
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9
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de Bruin A, Friddin MS, Elani Y, Brooks NJ, Law R, Seddon JM, Ces O. A transparent 3D printed device for assembling droplet hydrogel bilayers (DHBs). RSC Adv 2017. [DOI: 10.1039/c7ra09406j] [Citation(s) in RCA: 4] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/12/2022] Open
Abstract
We report a new approach for assembling droplet hydrogel bilayers (DHBs) using a transparent 3D printed device.
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Affiliation(s)
| | - Mark S. Friddin
- Department of Chemistry
- Imperial College London
- London
- UK
- Institute of Chemical Biology
| | - Yuval Elani
- Department of Chemistry
- Imperial College London
- London
- UK
- Institute of Chemical Biology
| | - Nicholas J. Brooks
- Department of Chemistry
- Imperial College London
- London
- UK
- Institute of Chemical Biology
| | - Robert V. Law
- Department of Chemistry
- Imperial College London
- London
- UK
- Institute of Chemical Biology
| | - John M. Seddon
- Department of Chemistry
- Imperial College London
- London
- UK
- Institute of Chemical Biology
| | - Oscar Ces
- Department of Chemistry
- Imperial College London
- London
- UK
- Institute of Chemical Biology
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