Rob W. Herman
San Diego, CA ***29
********@*****.***
Highlights and Skills
. Primer design and site-directed mutagenesis by overlap extension and
Quik-change PCR
. Standard molecular cloning and subcloning techniques
. E. coli transformations and screening for recombinant clones by
electrophoresis and DNA sequencing
. Sequencing with ABI3100 and sequence analysis using software such as
Chromas, Vector NTI and TeraTerm
. RNA isolation, purification and in vitro transcription
. Membrane protein expression in bacterial systems by fermentation and
transient transfection in mammalian cell cultures
. Membrane and protein isolation and purification via differential
centrifugation and affinity columns
. Trained to work in BSL 2 laboratories under aseptic conditions
Trained to handle mice; intraperitoneal injections, cardiac puncture,
euthanization
Fluorescence microscopy and analysis using Metamorph software
Professional Experience
Seattle Biomedical Research Institute, Seattle, WA
Research Technician II (January 2009-Present)
Flow cytometry and immunofluorescence assays to quantify malaria parasite
infectivity when exposed to specific drug concentrations.
Maintenance of malarial infection in mice via infected blood transfers.
Voluntary Leave of Absence (December 2006-December 2008)
Department of Chemistry and Biochemistry, UCLA, Los Angeles, CA
Research Associate II (June 2005-November 2006)
. Design and generation of mutant plasmids of proteins using site
directed mutagenesis.
. Protein expression using mammalian cell culture (transient
transfection).
. Purification of detergent-solubilized proteins using immunoaffinity
columns.
. Purification of native proteins from tissue using affinity columns
and differential centrifugation.
. Spin labeling of proteins for an EPR spectroscopy project focused
on determining inter-molecular distance measurements.
Scripps Institution of Oceanography, UCSD Marine Biology Division
Research Associate II (June 2004-April 2005)
. Extraction of RNA, DNA and proteins from wild type and mutant
cyanobacteria Synecococcus for microarray analysis, focusing on the
response from physiological and environmental stresses during
growth.
. Generation of gene knockouts and mutants using site-directed
mutagenesis.
. Laboratory safety coordinator and purchasing agent.
Department of Physiology, UCLA School of Medicine, Los Angeles, CA
Research Associate I (October 2001-March 2004)
. Design and generation of mutant genes via site-directed mutagenesis
and insertion into plasmids for senior members in a laboratory
focused on structure-function relations in voltage-gated ion
channels and transport proteins.
. Transcription and purification of mRNA from mutant clones for
microinjection into Xenopus oocytes.
. Preparation of DNA constructs and clones for mammalian cell
transfection.
National Genetics Institute, Los Angeles, CA
Laboratory Technician (May 2001-October 2001)
. Viral testing procedures of biological specimens.
. Trained in BSL 2 laboratories that specialized in quantification of
viral samples (HIV, HPV, Hep A, B and C and others).
Department of Chemistry, Syracuse University and University of
Connecticut
Laboratory Specialist (August 1998- March 2001)
. Manager of the Protein Expression and Isolation Laboratory.
. Membrane protein expression using mid-scale fermentation
bioreactors (10 L).
. Membrane-bound protein isolation and purification by differential
centrifugation and sucrose density gradients.
. Co-directed move of research facilities from Syracuse University to
University of Connecticut.
. Designed and developed a large-scale fermentation system using a
series of bioreactors (>50 L) to express native and mutant
proteins.
. Renovations and design of six laboratories in the University of
Connecticut, including a fully functional and contained Protein
Expression and Isolation Laboratory with a built-in autoclave and
large-scale bioreactor system.
. Purchasing agent for the research group.
Education
B.A. Earth Sciences, Adrian College, Adrian, MI, 1995
References available upon request.