KBI Biopharma

Managed and developed a team of CDMO research associates and scientists responsible for analytical testing of bioprocess development samples

SCIENTIST II (APR. 2023 – Present)

● Experienced in executing and developing methods to assess purity (SEC & RP-HPLC, Capillary Electrophoresis,  charge heterogeneity (IEX-HPLC, icIEF), impurities (HCP & ProA ELISAs, DNA), titer (affinity HPLC),  and glycan profiles (HILIC-UPLC-FLR)

● Lead analytical support for biological programs (MAbs and Fusion proteins) in both early phase (first in human) and late phase (Phase II to PPQ readiness)

● Authored and reviewed protocols, test methods, reports, data summaries and controlled documents in accordance with ICH guidelines and cGMP regulations

● Interfaced with pharmaceutical clients, upstream and downstream product development, and GMP manufacturing to ensure program deliverables and timelines were met

● Expedited timelines by improving data workflows (developed automated assay templates and data analysis reports) and standardized documentation (developed and trained company leads on automated data summary reports created using Visual Basic macros)

 
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Locus Biosciences

Engineer bacteria-killing bacteriophages with Cas3 nucleases as antibiotic alternatives.

Scientist II (MAR. 2021 – Present)

• High-throughput development team lead (11-member group); encompasses assay development, Hamilton automation engineering, automation operators, and related bioinformatics.

• Operations project lead to re-vamp organization using Lean Sigma 6 principles across four laboratories and two warehouse areas to maximize functional space and process efficiency. Successfully increased lab personnel capacity by 50% (11 individuals) through strategic space optimization.

• Selected as the unblinded scientist and subject matter expert for CROs during the Phase 2/3 ELIMINATE crPhage clinical trial

• Engineering product lead for CRISPR bacteriophage (crPhage) product to treat Klebsiella pneumoniae infections in partnership with CARB-X.

• Inter-department project lead for a major CapEx investment of $1.2 million to facilitate the automation of bacteriophage engineering. Lead author of project initiation form (PIF) and project charter.

• Completed the 9-week LEAD management program through the NextGen Center. Successful manager of 9 direct reports ranging from Research Technicians to Scientist IIs. Heavily involved in hiring process and acted as hiring manager for a scientist level position.

• Developed ELISA to quantify protein expression in murine and in vitro models

• Experience with all major forms of sequencing (Sanger, Illumina NGS, PacBio long read, ONR MinION). Led acquisition of PacBio Sequel IIe and personally optimized process for high-throughput gDNA extraction for NGS.

Scientist I (Nov. 2019 – FEB. 2021)

• Engineering project lead for the revision of the lead clinical CRISPR bacteriophage (crPhage) product to treat Escherichia coli urinary tract infections in partnership with BARDA.

• Implemented new DNA cloning and bacteriophage engineering strategies that reduced complexity and circumvented roadblocks. Listed inventor on two pending patents related to crPhage.

• Led a request for proposal (RFP) to identify a DNA synthesis vendor and managed vendor relationship to present. One outcome of this outsourcing was a year-over-year 10-fold increase in DNA constructs produced with a 6-fold reduction in cost per unit.

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WUSTL Department of EECE, 
Tae Seok Moon Laboratory

Graduate Student (Dec. 2014 – SEPT. 2019)

To help displace the widespread utilization of petrochemicals, my research combines genetic engineering, microbiology, and waste plant material to produce renewable fuels and chemicals for a more sustainable future. The core of my studies focusses on developing and applying genetic tools that facilitate the use of non-model organisms (i.e. those not commonly used in the lab) that have naturally evolved to excel at the conversion of plant material, particularly lignin, into valuable bio-commodities. These tools range from basic genetic elements for gene expression, to metabolite sensors for dynamic regulation of genetic circuits, to platforms for targeted genome engineering and metabolic flux modulation (CRISPR and CRISPRi).  These tools have been deployed to characterize and manipulate native genes and pathways related to lignin catabolism that can aid future engineering efforts.

  • Develop genetic tools and parts for non-model/understudied microbial species.

  • Experience with Escherichia coli, Synechocystis sp. PCC. 6803, Rhodococcus opacus PD630, and Corynebacterium glutamicum.

  • Goal is to produce sustainable bio-products from waste plant material (e.g. lignocellulose).

  • Awarded National Science Foundation Graduate Research Fellowship (NSF GRFP) for this work.

Lab Quartermaster (May 2016 – SEPT. 2019)

  • In charge of lab purchasing and inventorying.

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ESA Permit: 073-2013-01-002

ESA Permit: 073-2013-01-002

NOAA Hollings Internship

National Marine Fisheries Service - Panama City Beach, FL

May 2013 – Aug. 2013

  • Assessed the diet and trophic role of mesopredator sharks in coastal ecosystems (e.g. the Atlantic sharpnose shark).

  • Classified prey items to the lowest taxonomic level from 390 stomach samples.

  • First reported instance of Atlantic sharpnose sharks consuming juvenile loggerhead sea turtles.

  • Concluded that Atlantic sharpnose sharks occupy a different trophic or ecological level than previously determined, which has management implications.

  • Additionally assisted in conservation research related to loggerhead sea turtles and the endangered smalltooth sawfish.

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USC Department of Biology, Thomas J. Hilbish Laboratory

Oct. 2010 – May 2012

  • Investigated how the winter of 2009-‘10, one of the coldest in recent European history, affected the spatial distributions of two economically significant mussel species, Mytilus galloprovincialis and M. edulis, in Southwest England.

  • Utilized a polymerase chain reaction (PCR) assay to genotype mussel samples.

  • Compared population frequency data with temperature data to draw conclusions about the potential effects of climate change on sensitive ecosystems.

  • Awarded two grants for this research, one for the reseach effort and one for funding to present at the 2012 Benthic Ecology Conference.

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Duke University Marine Lab

May 2011 – June 2011

  • Investigated the concept of the Q10 thermal coefficient equation, which states that metabolic rate and chemical reactions can double or triple for every increase of 10 oC.
  • Collected barnacles (Balanus amphitrite) off the local boat dock and housed them in aquariums of varying temperatures (20-35 oC).
  • Concluded that barnacle feeding rate, and consequently metabolic rate, increased with water temperature.